structure and biological function of human 3-alpha hydroxysteroid
TRANSCRIPT
I
STRUCTURE AND BIOLOGICAL FUNCTION OF HUMAN 3-ALPHA HYDROXYSTEROID DEHYDROGENASE TYPE
3 IN BREAST CANCER
Thèse
BO ZHANG
Doctorat en Physiologie-Endocrinologie
Philosophiae Doctor (Ph.D.)
QUÉBEC, CANADA
© Bo Zhang, 2014
II
III
Résumé Court
RÉSUMÉ COURT
La 3-alpha hydroxystéroïde déshydrogénase de type 3 humaine (3α-HSD3) a un rôle
essentiel dans l’inactivation de la 5α-dihydrotestostérone (5α-DHT). Par une combinaison
de la mutagenèse, de la cinétique et de la cristallographie par rayon-X, nous démontrons
que la mutation de la Valine54 à la Leucine54 dans la 3α-HSD3 réduit sa capacité
d’inactivation de la 5α-DHT et améliore une activité 20-alpha hydroxystéroïde
déshydrogénase. Par ailleurs, la structure cristalline de la 3α-HSD3 en complexe avec la
5α-androstane-3,17-dione/épi-androstérone (A-dione/epi-ADT) a été obtenue par la co-
cristallisation, avec la 5α-DHT, ce qui implique que la 5α-DHT a des modes de liaison
alternative avec la 3α-HSD3. La suppression de l’expression de la 3α-HSD3 par des ARNsi
ne fait pas seulement qu’augmenter la concentration de la 5α-DHT dans les cellules MCF7,
mais elle diminue aussi la prolifération cellulaire des cellules MCF7 en présence de 5α-
DHT.
Le récepteur des estrogènes de type alpha (ERα) contrôle le développement sexuel et les
fonctions reproduction. Nous avons mis en place une méthode de purification du fragment
de l’ERα incluant son domaine de liaison à l’ADN et de son domaine de liaison au ligand
(DBD-LBD). La cristallogenèse préliminaire de l’ERα DBD-LBD en complexe avec les
éléments de réponse à l’estrogène a été effectuée. Par ailleurs, nous avons rapporté une
méthode de purification simple et efficace pour le domaine de liaison au ligand de l’ERα.
IV
V
Abstract
ABSTRACT
Human 3-alpha hydroxysteroid dehydrogenase type 3 (3α-HSD3) has an essential role in
the inactivation of androgen 5α-dihydrotestosterone (5α-DHT). By a combination of
mutagenesis, kinetics and X-ray crystallography, we demonstrate that the mutation of
Valine54 to Leucine54 in 3α-HSD3 reduces its 5α-DHT inactivation ability and enhances a
20-alpha hydroxysteroid dehydrogenase activity. Furthermore, the crystal structure of 3α-
HSD3 in complex with 5α-androstane-3,17-dione/epi-androsterone (A-dione/epi-ADT) is
obtained by co-crystallization with 5α-DHT, which implies that 5α-DHT has the alternative
binding mode within 3α-HSD3. Suppression of 3α-HSD3 expression by specific siRNA not
only increases 5α-DHT concentration in MCF7 cells, but also decreases MCF7 cell
proliferation in the presence of 5α-DHT.
Estrogen receptor alpha (ERα) controls sexual development and reproductive functions. We
establish a purification protocol of ERα fragment including its DNA binding domain and
ligand binding domain (DBD-LBD). Preliminary crystallogenesis of ERα DBD-LBD in
complex with estrogen response elements is carried out. Additionally, we report a simple
and efficient purification method for ERα LBD.
VI
VII
Résumé
RÉSUMÉ
L’estrogène 17β-estradiol (E2) stimule la prolifération des cellules du cancer du sein, alors
que la 5α-dihydrotestosterone (5α-DHT), qui est un androgène, prévient la croissance des
cellules du cancer du sein. La 3-alpha hydroxystéroïde déshydrogénase de type 3 humaine
(3α-HSD3) a un rôle essentiel dans le métabolisme des hormones stéroïdiennes,
particulièrement dans l’inactivation de l’androgène le plus actif, soit la 5α-DHT, ce qui fait
que la 3α-HSD3 agit comme un régulateur de pré-récepteur du récepteur des androgènes
(AR) dans le cancer de la prostate. Cependant, le rôle de la 3α-HSD3 dans les cellules
cancéreuses du cancer du sein n’a pas été assez étudié.
En combinant la mutagénèse et l’étude de la cinétique, nous démontrons que la mutation à
un seul point de la Valine54 à la Leucine54 (V54L), dans la 3α-HSD3 réduit
considérablement sa capacité de désactivation de la 5α-DHT et l’enzyme mutante acquiert
une activité de 20-alpha hydrostéroïde déshydrogénase accrue pour inactiver la
progestérone. De plus, nous avons analysé les structures cristallines des complexes 3α-
HSD3·NADP+·progestérone et 3α-HSD3 V54L·NADP
+·progestérone. Fait intéressant, la
progestérone dans l’enzyme sauvage possède deux différents modes de liaison, ce qui
indique que la site de liaison du stéroïde a une flexibilité considérable pour accommoder
différentes orientations du stéroïde. Cependant, la chaine latérale volumineuse de la Leu54
dans l’enzyme mutante restreint significativement le mouvement spatial du stéroïde et donc
permet seulement une orientation de liaison dans le site du substrat.
Par ailleurs, la structure cristalline de la 3α-HSD3 en complexe avec la 5α-androstane-3,17-
dione/épi-androstérone (A-dione/epi-ADT) a été obtenue par co-cristallisation avec la 5α-
DHT en présence de NADP+. Durant le processus de cristallisation, l’oxydoréduction de la
5α-DHT a produit un mélange de stéroïdes. L’A-dione et l’épi-ADT occupent la cavité de
deux monomères dans une unité asymétrique du cristal. Dans la cavité de l’enzyme, les
deux stéroïdes sont orientés l’un envers l’autre et les plans des deux stéroïdes sont
VIII
renversés d’environ 145°, ce qui démontre que la 5α-DHT a différentes façons de liaison
avec la 3α-HSD3 pour générer des produits. De plus, la suppression de l’expression de la
3α-HSD3 par des ARNsi spécifiques augmente la concentration de la 5α-DHT dans les
cellules MCF7 et, en conséquence, la suppression de l’expression de la 3α-HSD3 diminue
la prolifération des cellules MCF7 en présence de la 5α-DHT.
Le récepteur des estrogènes de type alpha (ERα) est un membre bien connu de la
superfamille des Récepteur Nucléaires (NRs). Par la liaison à la 17β-estradiol, l’ERα
contrôle le développement sexuel et les fonctions de reproduction. À cause des difficultés
rencontrées lors de l’expression de la protéine, de la purification et de la cristallisation, la
structure du ERα pleine longueur reste une tâche non tenues. Dans ce travail, nous avons
mis en place un protocole d’expression et de purification du fragment de l’ERα comprenant
son domaine de liaison à l’ADN et son domaine de liaison au ligand (DBD-LBD). La
cristallogenèse préliminaire de l’ERα DBD-LBD en complexe avec les éléments de réponse
à l’estrogène (EREs) a été effectuée, ce qui a généré des connaissances pour faciliter
l’acquisition de fins cristaux du complexe ERα DBD-LBD avec l’EREs. D’ailleurs, nous
avons rapporté une méthode simple et efficace pour la purification du domaine LBD de
l’ERα.
IX
Summary
SUMMARY
Estrogen 17β-estradiol stimulates the proliferation of breast cancer cells, whereas androgen
5α-dihydrotestosterone (5α-DHT) decreases breast cancer cell growth. Human 3-alpha
hydroxysteroid dehydrogenase type 3 (3α-HSD3) has an essential role in the steroid
metabolism, especially in the inactivation of the most potent androgen 5α-DHT, which
makes 3α-HSD3 acting as a pre-receptor regulator of androgen receptor (AR) in prostate
cancer. However, the role of 3α-HSD3 in breast cancer cells is short of investigations.
By combining mutagenesis and kinetic studies, we demonstrate that the mutation of
Valine54 to Leucine54 (V54L) in 3α-HSD3 significantly reduces its 5α-DHT inactivation
ability and the mutant enzyme acquires an enhanced 20-alpha hydroxysteroid
dehydrogenase activity to inactivate progesterone. Moreover, the crystal structures of the
3α-HSD3·NADP+·progesterone complex and the 3α-HSD3 V54L·NADP
+·progesterone
complex are hereby presented. Interestingly, progesterone in the wild type enzyme
possesses two different binding modes, which indicates the steroid binding pocket having
considerable flexibility to accommodate different orientations of a steroid. However, the
bulky side chain of Leu54 in the mutant enzyme significantly confines the spatial
movement of the steroid and thus allows only one binding orientation in the steroid binding
site.
Furthermore, the crystal structure of 3α-HSD3 in complex with 5α-androstane-3,17-
dione/epi-androsterone (A-dione/epi-ADT) is obtained by co-crystallization with 5α-DHT
in the presence of NADP+. During the crystallization process, the oxidoreduction of 5α-
DHT occurred and outputted a mixture of steroid metabolites. A-dione and epi-ADT are
found to occupy the cavities of two monomers in a crystal asymmetric unit, respectively. In
the steroid binding sites, two steroids are oriented upside down to each other and the planes
of two steroids are flipped about 145°, which shows the structural clues of 5α-DHT having
the alternative binding modes within 3α-HSD3 to generate products. In addition,
X
suppression of 3α-HSD3 expression by specific siRNA not only increases 5α-DHT
concentration in MCF7 cells, but also decreases MCF7 cell proliferation in the presence of
5α-DHT.
Estrogen receptor alpha (ERα) is a well-defined member of Nuclear Receptor superfamily
(NRs). Through binding to 17β-estradiol, ERα controls sexual development and
reproductive functions. Due to difficulties in protein expression, purification and
crystallization, the full-length ERα structure remains an unfulfilled task. In this work, we
establish an expression and purification protocol of ERα fragment including its DNA
binding domain and ligand binding domain (DBD-LBD). Preliminary crystallogenesis of
ERα DBD-LBD in complex with estrogen response elements (EREs) is carried out, which
provides basic knowledge to facilitate the acquisition of the fine crystals for ERα DBD-
LBD in complex with EREs. In addition, we report a simple and efficient purification
method for ERα LBD domain.
XI
TABLE OF CONTENTS
RÉSUMÉ COURT ............................................................................................................. III
ABSTRACT………………………………………………………………………………..V
RÉSUMÉ………………………………………………………………………...……….VII
SUMMARY………………………………………………………………………..……...IX
TABLE OF CONTENTS .................................................................................................. XI
LIST OF PUBLICATIONS .......................................................................................... XVII
LIST OF FIGURES ........................................................................................................ XIX
LIST OF TABLES .......................................................................................................... XXI
LIST OF ABBREVIATIONS ..................................................................................... XXIII
FOREWORD .............................................................................................................. XXVII
ACKNOWLEDGEMENTS ........................................................................................ XXIX
CHAPTER 1 INTRODUCTION ......................................................................................... 1
1.1 STEROID HORMONES AND HUMAN STEROIDOGENESIS ............................... 2
1.2 STEROID-RELATED CANCERS ............................................................................... 5
1.3 HUMAN 3ΑLPHA-HSD FAMILY .............................................................................. 7
1.4 HUMAN 3ΑLPHA-HSD3 ............................................................................................ 9
1.4.1 The biological functions of human 3α-HSD3 ..................................................... 9
1.4.2 The crystal structures of human 3α-HSD3 ........................................................ 10
1.4.3 The conserved NADP+ binding site .................................................................. 12
1.4.4 The steroid binding site ..................................................................................... 14
1.4.5 Catalytic mechanism ......................................................................................... 15
1.4.6 Kinetic features of human 3α-HSD3 ................................................................. 15
1.5 HUMAN NUCLEAR RECEPTORS .......................................................................... 16
1.6 HUMAN ESTROGEN RECEPTOR ALPHA ............................................................ 16
1.7 THE TOPICS OF THE RESEARCH PROJECTS ..................................................... 21
XII
CHAPTER 2 STRUCTURE-FUNCTION STUDY OF HUMAN 3-ALPHA
HYDROXYSTEROID DEHYDROGENASE TYPE 3 (3ΑLPHA-HSD3)
V54L MUTATION ..................................................................................... 23
2.0 PREFACE ................................................................................................................... 24
2.1 ABSTRACT ............................................................................................................... 26
2.2 INTRODUCTION ...................................................................................................... 27
2.3 MATERIALS AND METHODS ............................................................................... 28
2.3.1 Materials ........................................................................................................... 28
2.3.2 Site-directed mutagenesis ................................................................................. 29
2.3.3 Protein expression and purification .................................................................. 29
2.3.4 Crystallization ................................................................................................... 29
2.3.5 Data collection and structure determination ..................................................... 30
2.3.6 Kinetic analysis of the wild type and the mutant 3α-HSD3 ............................. 30
2.4 RESULTS ................................................................................................................... 31
2.4.1 Overall structure of the wild type and the mutant 3α-HSD3 ............................ 31
2.4.2 Conserved NADP+ binding ............................................................................... 31
2.4.3 The ternary complex of human 3α-HSD3·NADP+·progesterone ..................... 32
2.4.4 The ternary complex of human 3α-HSD3 V54L·NADP+·progesterone .......... 33
2.4.5 Kinetic study of the wild type and the mutant 3α-HSD3 .................................. 34
2.5 DISCUSSION ............................................................................................................. 34
2.6 FUNDING SOURCES ............................................................................................... 39
2.7 ACKNOWLEDGEMENTS........................................................................................ 39
2.8 REFERENCES ........................................................................................................... 40
CHAPTER 3 STRUCTURE CLUES OF 5ΑLPHA-DHT ALTERNATIVE BINDING
WITHIN HUMAN 3ΑLPHA-HSD3 AND THE ROLE OF THE
ENZYME IN BREAST CANCER ............................................................ 59
3.0 PREFACE ................................................................................................................... 60
3.1 ABSTRACT ............................................................................................................... 62
3.2 INTRODUCTION ...................................................................................................... 63
3.3 MATERIALS AND METHODS ............................................................................... 64
3.3.1 Materials ........................................................................................................... 64
3.3.2 Protein purification and crystallization ............................................................. 65
XIII
3.3.3 Data collection and structure determination ...................................................... 65
3.3.4 The oxidoreduction assay of steroids and the GC/MS analysis ........................ 66
3.3.5 Cell culture ........................................................................................................ 66
3.3.6 siRNA synthesis and transfection ...................................................................... 66
3.3.7 Quantitative real-time RT-PCR ......................................................................... 67
3.3.8 Determination of 5α-DHT levels by Elisa assay ............................................... 67
3.3.9 Cell proliferation assay ...................................................................................... 67
3.4 RESULTS ................................................................................................................... 68
3.4.1 Crystal growth of human 3α -HSD3 in complex with A-dione/epi-ADT and 4-
dione .................................................................................................................. 68
3.4.2 Overall structures of human 3α-HSD3 in complex with A-dione/epi-ADT and
4-dione .............................................................................................................. 69
3.4.3 Human 3α-HSD3 in complex with A-dione/epi-ADT ...................................... 69
3.4.4 Human 3α-HSD3 in complex with 4-dione ....................................................... 70
3.4.5 3α-HSD3 expression and siRNA specific knockdown in MCF7 cells .............. 71
3.4.6 Suppression of 3α-HSD3 expression increases 5α-DHT concentration in MCF7
cells ................................................................................................................... 72
3.4.7 Suppression of 3α-HSD3 expression decreases MCF7 cell proliferation in the
presence of 5α-DHT .......................................................................................... 72
3.5 DISCUSSION ............................................................................................................. 72
3.6 FUNDING SOURCES ................................................................................................ 75
3.7 ACKNOWLEDGEMENTS ........................................................................................ 76
3.8 REFERENCES ............................................................................................................ 77
CHAPTER 4 PURIFICATION AND PRELIMINARY CRYSTALLOGENESIS OF
HUMAN ESTROGEN RECEPTOR ALPHA .......................................... 97
4.0 PREFACE ................................................................................................................... 98
4.1 EXPRESSION, PURIFICATION AND PRELIMINARY CRYSTALLOGENESIS
OF HUMAN ESTROGEN RECEPTOR ALPHA DBD-LBD ................................... 99
4.1.1 Abstract ........................................................................................................... 100
4.1.2 Introduction ..................................................................................................... 101
4.1.3 Methods ........................................................................................................... 102
4.1.3.1 Plasmids construction ......................................................................... 102
XIV
4.1.3.2 Site-directed mutagenesis of ERα C530A .......................................... 102
4.1.3.3 Protein expression and purification .................................................... 102
4.1.3.4 Solubility test ...................................................................................... 103
4.1.3.5 Western blot analysis .......................................................................... 104
4.1.3.6 Preliminary test of crystallization ....................................................... 104
4.1.4 Results and discussion .................................................................................... 104
4.1.4.1 Construction, expression and solubility test of ERα DBD-LBD........ 104
4.1.4.2 Purification of ERα DBD-LBD .......................................................... 105
4.1.4.3 Preliminary crystallogenesis of ERα DBD-LBD ............................... 106
4.1.5 Perspective ...................................................................................................... 107
4.1.6 Acknowledgements ......................................................................................... 107
4.1.7 References ....................................................................................................... 108
4.2 A SIMPLE AND EFFICIENT PURIFICATION METHOD FOR HUMAN
ESTROGEN RECEPTOR ALPHA LBD ................................................................ 117
4.2.1 Abstract ........................................................................................................... 118
4.2.2 Introduction ..................................................................................................... 119
4.2.3 Methods .......................................................................................................... 120
4.2.3.1 Site-directed mutagenesis of ERα LBD C530A ................................. 120
4.2.3.2 Protein expression and purification .................................................... 120
4.2.3.3 Solubility test ...................................................................................... 121
4.2.4 Results and discussion .................................................................................... 121
4.2.4.1 Expression and solubility test of ERα LBD ....................................... 121
4.2.4.2 Purification of ERα LBD .................................................................... 122
4.2.5 Acknowledgements ......................................................................................... 123
4.2.6 References ....................................................................................................... 124
CHAPTER 5 CONCLUSIONS ....................................................................................... 129
5.1 STRUCTURE-FUNCTION STUDY OF HUMAN 3ΑLPHA-HSD3 SINGLE POINT
MUTATION V54L ENHANCING THE 20ΑLPHA-HSD ACTIVITY ................. 131
5.2 STRUCTURAL CLUES OF 5ΑLPHA-DHT ALTERNATIVE BINDING WITHIN
HUMAN 3ΑLPHA-HSD3 AND DOWN-REGULATION OF 3ΑLPHA-HSD3
DECREASING BREAST CANCER CELL GROWTH .......................................... 132
XV
5.3 PURIFICATION AND PRELIMINARY CRYSTALLOGENESIS OF HUMAN
ESTROGEN RECEPTOR ALPHA DBD-LBD ....................................................... 134
5.4 A SIMPLE AND EFFICIENT PURIFICATION METHOD FOR HUMAN
ESTROGEN RECEPTOR ALPHA LBD ................................................................. 135
5.5 FUTURE TOPICS .................................................................................................... 136
CHAPTER 6 REFERENCES (FOR INTRODUCTION) ............................................. 137
XVI
XVII
LIST OF PUBLICATIONS
1. Bo Zhang, Dao-Wei Zhu, Xiao-Jian Hu, Ming Zhou, Peng Shang, Sheng-Xiang Lin.
(2014). Human 3-alpha hydroxysteroid dehydrogenase type 3 (3α-HSD3): the V54L
mutation restricting the steroid alternative binding and enhancing the 20α-HSD
activity (Journal of Steroid Biochemistry and Molecular Biology 141 (2014) 135-
143).
2. Bo Zhang, Xiao-Jian Hu, Xiao-Qiang Wang, Dao-Wei Zhu, Peng Shang, Fernand
Labrie, Sheng-Xiang Lin. (2014). Human 3-alpha hydroxysteroid dehydrogenase
type 3: structural clues of 5α-DHT alternative binding and enzyme down-regulation
decreasing breast cancer cell growth (to be submitted).
3. Bo Zhang, Sheng-Xiang Lin. Expression, purification and preliminary
crystallogenesis of human estrogen receptor alpha DBD-LBD (in preparation).
4. Bo Zhang, Jean-François Thériault, Dao-Wei Zhu, Sheng-Xiang Lin. A simple and
efficient purification method for human estrogen receptor alpha LBD (in
preparation).
XVIII
XIX
LIST OF FIGURES
Figure 1.1 Steroid core and its numbering system ............................................................... 2
Figure 1.2 Partial representation of the steroidogenesis ...................................................... 5
Figure 1.3 The overall structure of human 3α-HSD3 with cofactors and steroids ............ 10
Figure 1.4 The detailed interactions between 3α-HSD3 and NADP+ ................................ 12
Figure 1.5 The detailed interactions in the steroid binding site of 3α-HSD3 .................... 13
Figure 1.6 Proposed catalytic mechanism of 3α-HSDs ..................................................... 14
Figure 1.7 Structural organization of ERα ......................................................................... 17
Figure 1.8 ERα in complex with ligands and coregulators ................................................ 19
Figure 2.1 Structure of the 3α-HSD3·NADP+·progesterone complex .............................. 49
Figure 2.2 Structure of the 3α-HSD3 V54L·NADP+·progesterone complex .................... 52
Figure 2.3 Presence of the reduced form of the cofactor NADPH within the purified
protein samples of the wild type 3α-HSD3 and the V54L mutant .................. 54
Figure 2.4 Superposition of the steroid binding sites of human 3α-HSD3 related structures
......................................................................................................................... 55
Figure 3.1 The oxidoreduction of 5α-DHT catalyzed by human 3α-HSD3 in the presence
of cofactors ...................................................................................................... 85
Figure 3.2 Structure of the 3α-HSD3·NADP+·A-dione/epi-ADT complex ...................... 86
Figure 3.3 The oxidation of testosterone catalyzed by human 3α-HSD3 in the presence of
NADP+ ............................................................................................................ 89
Figure 3.4 Structure of the 3α-HSD3·NADP+·4-dione complex ....................................... 90
Figure 3.5 Human 3α-HSD3 expression and knockdown by siRNA in MCF7 cells ........ 92
Figure 3.6 Suppression of 3α-HSD3 in MCF7 cells enhanced 5α-DHT-mediated
inhibition of cell growth .................................................................................. 93
Figure 3.7 Superposition of the steroid binding sites of the related 3α-HSD3 structures . 94
XX
Figure 4.1.1 The constructions of Human ERα DBD-LBD recombinant plasmids ........ 112
Figure 4.1.2 The verification of ERα DBD-LBD expression in Rosetta2 (DE3) cells ... 113
Figure 4.1.3 Expression results of ERα DBD-LBD (179-595aa) in Rosetta2 (DE3) cells
...................................................................................................................... 114
Figure 4.1.4 Purification results of ERα DBD-LBD (179-595aa) .................................. 115
Figure 4.1.5 Preliminary crystallogenesis of ERα DBD-LBD (179-554aa) ................... 116
Figure 4.2.1 Expression result of ERα LBD ................................................................... 126
Figure 4.2.2 Solubility test of ERα LBD ......................................................................... 127
Figure 4.2.3 Purification result of ERα LBD .................................................................. 128
XXI
LIST OF TABLES
Table 2.1 Data collection and refinement statistics ........................................................... 46
Table 2.2 Steady-state kinetic parameters for 5α-DHT and progesterone reduction
catalyzed by the wild type (WT) 3α-HSD3 and the Val54Leu (V54L) mutant in
the presence of NADPH ..................................................................................... 48
Table 3.1 Data collection and refinement statistics ........................................................... 83
XXII
XXIII
LIST OF ABBREVIATIONS
3α-diol 5α-androstane-3α,17β-diol
3α-HSD 3α-hydroxysteroid dehydrogenase
3α-HSD3 3α-hydroxysteroid dehydrogenase type 3
3(α/β)-HSE 3(α/β)-hydroxysteroid dehydrogenase epimerase
3β-diol 5α-androstane-3β,17β-diol
3β-HSD 3β-hydroxysteroid dehydrogenase/Δ5-Δ
4-isomerase
3D three dimensions
4-dione 4-androstene-3,17-dione
5α-DHT 5α-dihydrotestosterone
5α-Rs 5α-reductase
17-OH-Preg 17-hydroxypregnenolone
17-OH-Prog 17-hydroxyprogesterone
17β-HSD 17β-hydroxysteroid dehydrogenase
20α-HSD 20α-hydroxysteroid dehydrogenase
20α-OHProg 20α-hydroxy-progesterone
Å angstrom
aa amino acids
A-dione 5α-androstane-3,17-dione
ADT androsterone
AF activation function region
AKR aldo-keto reductase
AR androgen receptor
β-DDM dodecyl-β-D-maltoside
β-OG β-octyl glucoside
BPH benign prostatic hyperplasia
BSA bovine serum albumin
C12E8 octaethylene glycol monododecyl ether
CHOL cholesterol
CORT cortisol
CV column volume
XXIV
DBD DNA binding domain
DD4 dihydrodiol dehydrogenase isoform 4
DES diethylstilbestrol
DHEA dehydroepiandrosterone
DHEAS dehydroepiandrosterone sulfate
DHT dihydrotestosterone
DMEM Dulbecco’s Modified Eagle’s Medium
DTT dithiothreitol
E1 estrone
E1S estrone sulfate
E2 17β-estradiol
EDTA ethylenediaminetetraacetic acid
epi-ADT epi-androsterone
ER estrogen receptor
ERα estrogen receptor alpha
ERβ estrogen receptor beta
EREs estrogen response elements
FBS fetal bovine serum
GABAA γ-aminobutyric acid type A
GC/MS gas chromatography/mass spectrometer
GR glucocorticoid receptor
GST glutathione S-transferase
HAT histone acetyltransferase
HDAC histone deacetylase
HPLC high performance liquid chromatography
IPTG isopropyl-β-D-thiogalactopyranoside
Kcat the catalytic rate constant
Km the Michaelis-Menten constant
kDa kilodalton
LB lysogeny broth
LBD ligand binding domain
XXV
M molar
MES 2-(N-morpholino)ethanesulfonic acid
mg milligram
min minute
ml milliliter
mM millimolar
MR molecular replacement
MTT 3-(4, 5-dimethylthiazol-2-yl)-2, 5-diphenyltetrazolium bromide
NAD nicotinamide adenine dinucleotide
NADH nicotinamide adenine dinucleotide reduced form
NADP nicotinamide adenine dinucleotide phosphate
NADPH nicotinamide adenine dinucleotide phosphate reduced form
NC negative control
NcoR nuclear receptor corepressor
NDSB non detergent sulfobetaines
ng nanogram
nl nanoliter
NLS nuclear localization sequence
nM nanomolar
nm nanometer
NR nuclear receptor
Nrf2 nuclear factor erythroid-2 related factor 2
OD optical density
OHT 4-hydroxytamoxifen
P450arom aromatase
P450c17 17α-hydroxylase/17,20-lyase
P450scc cholesterol side-chain cleavage
PBS phosphate buffer saline
PCR polymerase chain reaction
PEG polyethylene glycol
pg picogram
XXVI
PMSF phenylmethylsulfonyl fluoride
PPARγ peroxisome proliferator-activated receptor gamma
PREG pregnenolone
PROG progesterone
q-RTPCR quantitative real-time PCR
RMSD root mean square deviations
RXRα retinoid X receptor alpha
SDR short-chain dehydrogenase/reductase
SDS-PAGE sodium dodecyl sulphate-polyacrylamide gel electrophoresis
sec second
SERM selective estrogen receptor modulator
siRNA small interfering RNA
SMRT silencing mediator for retinoid and thyroid hormone receptor
SRC steroid receptor coactivator
STS steroid sulfatase
SULT sulfotransferase
Testo testosterone
TF transcription factor
TIM triose-phosphate isomerase
TLC thin layer chromatography
TR thyroid receptor
Tris tris(hydroxymethyl)aminomethane
μg microgram
μl microliter
μM micromolar
WT wild type
XXVII
Foreword
FOREWORD
This thesis includes four scientific manuscripts prepared during my graduate study. One
article has been published in the Journal of Steroid Biochemistry and Molecular Biology,
the second will be submitted soon, and the two others are in preparation.
In chapter 1 (Introduction), the general ideas on human steroidogenesis and the related
enzymes, steroid-related cancers, human 3-alpha hydroxysteroid dehydrogenase (3α-HSD)
family and 3α-HSD3, human nuclear receptors and estrogen receptor alpha are briefly
reviewed.
Chapter 2 includes one manuscript on the structure-function study of human 3α-HSD3
V54L mutation: Bo Zhang, Dao-Wei Zhu, Xiao-Jian Hu, Ming Zhou, Peng Shang, Sheng-
Xiang Lin. (2014). Human 3-alpha hydroxysteroid dehydrogenase type 3 (3α-HSD3): the
V54L mutation restricting the steroid alternative binding and enhancing the 20α-HSD
activity (Journal of Steroid Biochemistry and Molecular Biology 141 (2014) 135-143). In
this paper, I carried out all the experimental studies, solved the crystal structures and wrote
the manuscript. Dr. Sheng-Xiang Lin and I designed the study.
Chapter 3 includes one manuscript on the structure clues of 5α-DHT alternative binding
within human 3α-HSD3 and the role of the enzyme in breast cancer: Bo Zhang, Xiao-Jian
Hu, Xiao-Qiang Wang, Dao-Wei Zhu, Peng Shang, Fernand Labrie, Sheng-Xiang Lin.
(2014). Human 3-alpha hydroxysteroid dehydrogenase type 3: structural clues of 5α-DHT
alternative binding and enzyme down-regulation decreasing breast cancer cell growth (to be
submitted). In this paper, I carried out all the experimental studies except for the work
indicated below. I and Dr. Xiao-Jian Hu solved the crystal structure of the 3α-
HSD3·NADP+·A-dione/epi-ADT complex. I solved the crystal structure of the 3α-
HSD3·NADP+·4-dione complex. Mr. Xiang-Qiang Wang and I used the ELISA kit to
detect the 5α-DHT concentration. The q-RTPCR platform and the bioanalytical platform
XXVIII
(Centre Hospitalier Universitaire (CHU) de Quebec Research Center (CHUL) and Laval
University, Québec) offered the services for the q-RTPCR analysis and the GC/MS analysis.
I wrote the manuscript. Dr. Sheng-Xiang Lin and I designed the study.
Chapter 4 includes two manuscripts. (1) The first manuscript is focused on purification and
preliminary crystallogenesis of human ERα DBD-LBD: Bo Zhang, Sheng-Xiang Lin.
Expression, purification and preliminary crystallogenesis of human estrogen receptor alpha
DBD-LBD (in preparation). In this paper, I carried out all the experimental studies and
wrote the manuscript. Dr. Sheng-Xiang Lin and I designed the study. (2) The second
manuscript is focused on an efficient purification method for ERα LBD: Bo Zhang, Jean-
François Thériault, Dao-Wei Zhu, Sheng-Xiang Lin. A simple and efficient purification
method for human estrogen receptor alpha LBD (in preparation). In this paper, I carried out
the experimental studies and wrote the manuscript. Mr. Jean-François Thériault as a
summer student prepared some SDS-PAGE gels. Dr. Sheng-Xiang Lin, Dr. Dao-Wei Zhu
and I designed the study.
Chapter 5 contains the conclusions.
Chapter 6 contains the references for chapter 1.
XXIX
Acknowledgements
ACKNOWLEDGEMENTS
I express the deepest acknowledgement to Dr. Sheng-Xiang Lin, the supervisor of my Ph.D.
study at Laval University. Dr. Lin guided me into the field of the structural biology,
especially into the field of X-ray crystallography. This research field has been my pursuit
for long time. It is my honor to study in Dr. Lin’s laboratory, which has accumulated
experiences in biochemistry and X-ray crystallography for twenty years. Dr. Lin has a
broad vision in basic science and his open mind for discussions often benefits me in many
aspects. His enthusiasm for medical research and conscientious working attitude will
significantly affect me in my future career.
I also express the deepest acknowledgement to Dr. Peng Shang, the supervisor of my Ph.D.
study in China. It was Dr. Peng Shang who offered me the opportunity to transform my
research field from computational biology to experimental biology. In Dr. Peng Shang’s
laboratory, I received the basic training on molecular cloning and protein purification,
which greatly facilitated my subsequent study. His open mind and professional knowledge
affected me continuously. Without his support, I can hardly fulfill my study abroad.
I express my acknowledgement to Dr. Dao-Wei Zhu. He taught me a lot of practical
methods in protein purification and shared his valuable experiences in crystallogenesis.
Without his help, the research project could be more difficult to be carried through.
I also express my acknowledgement to Dr. Ming Zhou. She guided me in enzyme kinetic
studies and instructed me many useful skills in protein purification and crystallogenesis. I
was impressed by her capability to identify the problems and rapidly to solve them.
I thank very much Dr. Pei-min Rong, who taught me the basic skills of Western-blot. After
he retired from the research center, Dr. Rong also gave me a lot of help in daily lives.
XXX
I express my special thanks to Dr. Xiao-Jian Hu. During his visiting in our laboratory, Dr.
Hu gave me basic training in crystal data collection and X-ray crystallography. During the
attempts to obtain the crystal structures, we had many discussions together. He always
patiently answered any questions from me.
I thank very much Dr. Donald Poirier, who not only kindly offered us some chemicals that
we did not have in our laboratory, but also gave the professional answers and suggestions
for a number of questions from me.
I also express my thanks to Dr. Van Luu-The and Dr. Fernand Labrie, who provided us the
radioactive progesterone and the plasmid of human 3-alpha hydroxysteroid dehydrogenase
type 3.
I express my acknowledgements to Dr. Juliette-A. Aka, Dr. Mausumi Mazumdar, Dr.
Chen-Yan Zhang and Dr. Ying Wang. They showed me some basic knowledge in cellular
functional experiments and X-ray crystallography. I can’t forget that we had so many
meaningful discussions on research topics.
I express my thanks to Dr. Preyesh Stephen, who revised the manuscripts of chapters 1, 3
and 4 in this thesis. I express my thanks to Dr. Kathryn Leake, who revised the manuscript
of chapter 4 in this thesis. I also specially thank Mr. Jean-François Thériault for the
translation of the abstract and the summary for this thesis from English to French. Mr.
Thériault and I had numerous discussions on the research. When I met any problems, he
always helped me without hesitation.
I want to express my thanks to Dr. Feng-Fei Huang for her helpful instruction on the
method of co-immunoprecipitation. I also thank Dr. Jing-Bao Li, Dr. Sheng-Meng Di and
Dr. Wei-ning Niu for the basic training to me on molecular cloning and protein purification.
I thank Dr. Jiong Chen and Miss Wei-Qi Wang for ordering the plasmid of human estrogen
receptor alpha and several fragments of siRNA from China and sending them by post to
Canada.
XXXI
I also express my acknowledgements to Mr. Yi Han, Miss Mouna Zerradi, Mr. Xiao-Qiang
Wang, Mr. Le-Yi Lin, Mr. Jian Song, Miss Dan Xu, Miss Hui Han, Dr. Ai-Rong Qian, Mr.
Zhe Wang, Mr. Peng-Fei Yang, Miss Li-Fang Hu, Miss Chong Ding, Mr. Yong-Liang
Wang and Mr. Zhen-Kun Sun. I have received a lot of help and many useful suggestions
from them.
I want to express my acknowledgements to Ms. Nathalie Paquet, Mr. Patrick Bélanger and
Mr. Ronald Maheux for their professional services, who are from the q-RTPCR platform,
the bioanalytical platform and the image-analysis platform (Centre Hospitalier
Universitaire (CHU) de Quebec Research Center (CHUL) and Laval University, Québec),
respectively.
I express my thanks to PROTEO (The Quebec Network for Research on Protein Function,
Structure, and Engineering) and Dr. Albert Berghuis’ laboratory at McGill University,
which offered the X-ray crystallography facilities for our initial X-ray datasets collection. I
also thank LRL-CAT at the Advanced Photon Source, Argonne National Laboratory, and at
the CMCF facility, Canadian Light Source, in which X-ray datasets were collected.
I thank China Scholarship Council (CSC) for supporting my graduate study at Laval
University by providing a national scholarship. I also thank the grant (MOP 97917) to Dr.
Sheng-Xiang Lin and collaborators by CHIR (Canadian Institute of Health Research).
Finally, I express my deepest gratitude for the spiritual support from my parents and my
sisters. Their great love has always given me the courage and the strength to face the
difficulties.
XXXII
1
CHAPTER 1 INTRODUCTION
2
1.1 STEROID HORMONES AND HUMAN STEROIDOGENESIS
Steroid hormones are originated from the endogenous and exogenous cholesterol and are
sharing a cyclopentanoperhydrophenanthrene nucleus (Figure 1.1), which include sex
steroids (estrogens, androgens and progestins), mineralocorticoids and glucocorticoids 1.
They have diverse physiological functions, especially involving into the regulation of
human reproduction 2; 3
. Cholesterol is characterized by 27 carbon atoms. Steroids have
been classified into several major classes based on their chemical structures, of which
cholestanes possess 27 carbons (such as cholesterol), cholanes possess 24 carbons (such as
cholic acid), pregnanes possess 21 carbons (such as progesterone), androstanes have 19
carbons (such as testosterone) and estranes have 18 carbons (such as estradiol) 4.
Steroid core Standard numbering system
Figure 1.1 Steroid core and its numbering system
Sex steroids can be synthesized in gonadal organs such as testis and ovary, which are
released into the blood circulation and transferred to distant target cells through endocrine
pathway 5. Besides, a large amount of sex steroids are synthesized in peripheral tissues
from their inactive precursors, which are dehydroepiandrosterone (DHEA) and DHEA-
sulfate (DHEA-S) from the adrenal gland 5; 6
. It is noteworthy that, in men, about 50% of
androgens are synthesized from DHEA in peripheral tissues; while in women, about 75%
or nearly 100% estrogens are synthesized before or after menopause in peripheral tissues,
3
respectively 7. Through diffusing into the target cells and binding to the nuclear hormone
receptors, sex steroids initialize the activation or repression of their target gene
transcriptions.
Different classes of enzymes are involved into the steroidogenesis and steroid metabolism 1
(Figure 1.2). In the following paragraphs, several key enzymes related to the
steroidogenesis of sex steroids will be introduced briefly.
Human steroid sulfotransferase (SULT) uses the sulfonate anion from 3’-
phosphoadenosine-5’-phosphosulfate and catalyzes the transformations of steroids to their
inactive sulfated forms 8; 9
. Particularly, estrogen sulfotransferase (gene named SULT1E1)
will sulfonate the 3-hydroxyl group of estrogen 4; 10
. Besides, steroid sulfatase (STS) is
responsible for the conversion of sulfated steroids to the active steroids 11; 12
. Steroid
sulfatase deficiency leads to the X chromosome-linked ichthyosis and the impairment of
placental estrogen synthesis 4; 13
.
The family of human 17β-hydroxysteroid dehydrogenases (17β-HSDs) catalyzes the
reduction of 17-ketosteroids or the oxidation of 17β-hydroxysteroids 10; 14; 15; 16
. To date, 15
different 17β-HSDs have been identified and they belong to the short-chain
dehydrogenase/reductase (SDR) superfamily, except for type 5 17β-HSD, which is a
member of the aldo-keto reductase (AKR) superfamily. These enzymes can be divided into
two groups that one group uses NADPH as the cofactor for reduction (such as types 1, 3, 5
and 7 of 17β-HSD), and the other group uses NAD+ as the cofactor for oxidation (such as
types 2, 4, 6 and 8 of 17β-HSD) 4. These isoenzymes differ in tissue distribution, catalytic
mechanism, substrate specificity and physiological functions 10; 17
.
Human 3β-hydroxysteroid dehydrogenases (3β-HSDs) catalyze both the conversion of
steroidal 3β-hydroxyl group to 3-keto group and the isomerisation of the double bond from
Δ5-steroid to
Δ
4-steroid
18; 19. In human, two 3β-HSDs are identified. 3β-HSD1 is expressed
in placenta and peripheral tissues. 3β-HSD2 is primarily expressed in gonads and adrenal
glands 20
.
4
5
Figure 1.2 Partial representation of the steroidogenesis
The name and abbreviation of steroids and enzymes are listed in the section of “LIST OF
ABBREVIATIONS” in the thesis. (This figure is from Poirier D, Expert Opin. Ther.
Patents, 2010.)
Human 5α-reductases are membrane-associated enzymes that preferentially catalyze the
transformation of testosterone (Testo) to 5α-DHT, which act as important regulators of
androgen receptor 21
. Two major isoenzymes are found in this family, and type 2 5α-
reductase is predominantly expressed in male genital skin, epididymis and prostate to
generate the most potent androgen 5α-DHT 22; 23
.
Aromatase (P450arom) is the only known enzyme in vertebrates to be responsible for the
biosynthesis of estrogens from androgens, and it catalyzes three sequential reactions of two
C19 steroids (4-dione and Testo) to produce their corresponding C18 steroids (estrone and
estradiol) with a phenolic A-ring 24; 25; 26
.
Human 3-alpha hydroxysteroid dehydrogenase family (3α-HSD) possesses different
degrees of 3-keto-, 17-keto-, and 20-ketosteroid reductase activities 27; 28
. This family
contains four isoenzymes, and belongs to the aldo-keto reductase (AKR) superfamily. In
particular, human 3α-HSD type 3 (3α-HSD3) has an essential role to inactivate the most
potent androgen 5α-dihydrotestosterone (5α-DHT), which behaves as a pre-receptor
regulator of androgen receptor (AR) in prostate cancer 29
. However, androgen 5α-DHT has
been shown to prevent breast cancer cell growth. Very few studies have been conducted to
investigate the role of 3α-HSD3 in breast cancer. Therefore, the structure-function study of
human 3α-HSD3 in breast cancer is the major research topic of this thesis and enzymes in
this family will be introduced in details in the subsequent sections.
1.2 STEROID-RELATED CANCERS
Unlike chemicals or viruses induced cancers, steroid-related cancers involved in breast,
ovary, prostate, testis, thyroid, endometrium and osteosarcoma share a distinct mechanism
6
for carcinogenesis 30; 31
. Steroids have an outstanding role to stimulate the cell division and
proliferation, and thus the random genetic errors are accumulated during these processes,
which will lead to a malignant phenotype 32
. The candidate genes of steroid-related cancers
are involved in the endocrine pathway, tumor suppressor genes and oncogenes. For
examples, human 17β-hydroxysteroid dehydrogenase type 1 gene (HSD17B1) and human
aromatase gene (CYP19) are involved in the endocrine pathway related to breast cancer;
BRCA1 and BRCA2 are responsible for repairing DNA, which are two tumor suppressor
genes and mutations in these two genes significantly increase risks for developing breast
cancer and ovarian cancer 32
.
Breast cancer and prostate cancer are two common steroid-related cancers for women and
men, respectively. According to the statistics of the American Cancer Society
(http://www.cancer.org/), about 12% women in US will develop breast cancer during the
lifetime, and about 232,340 new cases of breast cancer will be diagnosed in women for the
year of 2013 in US. Breast cancer is the second leading cause of death from cancer in
women, after lung cancer. In addition, prostate cancer is the second leading cause of death
from cancer in American men, about 17% men in US will develop prostate cancer during
the lifetime, and about 238,590 new cases of prostate cancer will be diagnosed for the year
of 2013 in US. According to the statistics of the Canadian Cancer Society
(http://www.cancer.ca), breast cancer is the second leading cause of death from cancer in
Canadian women, and it is estimated that 26% of all new cancer cases in women will be
diagnosed with breast cancer for the year of 2013; in addition, prostate cancer is the third
leading cause of death from cancer in Canadian men, and it is estimated that 25% of all new
cancer cases in men will be diagnosed with prostate cancer for the year of 2013.
Sex steroid such as 17β-estradiol has a role to stimulate cell proliferation and promote
breast cancer development 33; 34
. The rapid rate of cell proliferation can initiate mutations
due to the reduced duration of DNA repair, and increase the risk of cancer-causing
mutations 35; 36
. In particular, after menopause of female, estrogens are predominantly
produced from adrenal and ovarian androgens by aromatase in the peripheral tissues such
as skin, fat and muscle 37
. The genetic variations of aromatase are associated with an
increased risk of developing breast cancer 38
. On the other side, sex steroids such as Testo
7
and 5α-DHT play a significant role in normal prostate development and prostate cancer 39
.
The studies of Huggins and Hodges show that prostate cancer is inhibited by androgen
deprivation therapy and activated by androgen injection 40
. Particularly, the development of
normal prostate and benign prostatic hyperplasia (BPH) depends on androgen 5α-DHT. In
prostate, Testo is irreversibly catalyzed to 5α-DHT by type 2 5α-reductase, and the most
potent androgen 5α-DHT binds within androgen receptor to stimulate the cell proliferation
31; 41; 42. The genetic mutations for type 2 5α-reductase and androgen receptor are found to
suppress or block the normal prostate development and are associated with increased risk of
prostate cancer 39; 43; 44; 45
.
1.3 HUMAN 3ΑLPHA-HSD FAMILY
Human 3-alpha hydroxysteroid dehydrogenase family (3α-HSD) includes four isoenzymes
(types 1, 2, 3 and 4), which belongs to the aldo-keto reductase (AKR) superfamily. These
enzymes possess varying degrees of 3-keto-, 17-keto-, and 20-ketosteroid reductase
activities to catalyze the inactivation of androgens, estrogens, progestins, and bile acid
precursors 10; 27; 29; 46
. Human 3α-HSD types 1, 2, 3 and 4 are also named to AKR 1C4, 1C3,
1C2 and 1C1, respectively 47
. The genes of these four enzymes are clustered on
chromosome 10p14-15 and consist of nine exons 28; 48
. The protein sequences of these four
enzymes have more than 81% identity and show differential tissue distributions 27; 28; 49; 50
.
These enzymes adopt a well known triose-phosphate isomerase (TIM) barrel motif or an
(α/β)8-barrel motif and share a conserved cofactor binding site 51; 52; 53; 54
. The substrate
binding site is located at the C-terminal end of the barrel 52
. 3α-HSDs prefer NADPH over
NADH, and NADP is mostly in its reduced form in metabolically active cells 55
.
Human 3α-HSD1 (AKR1C4) is almost exclusively expressed in human liver 27
, which is
also known as hepatic dihydrodiol dehydrogenase isoform 4 (DD4) or chlordecone
reductase 56; 57
. This enzyme converts a keto group to a hydroxy group, which probably has
a significant role in the detoxification of compounds containing a keto group 50
. Besides,
working in concert with 5α/5β-reductases, 3α-HSD1 catalyzes 3-keto steroids to 3α-
hydroxy steroids, which could maintain the homeostasis of steroids and facilitate the final
elimination of steroids by sulfotransferase or glucuronosyl transferase 50; 58
.
8
Human 3α-HSD2 (also named 17β-HSD5 or AKR1C3) is expressed dominantly in prostate
and mammary glands. It plays a major role of Testo biosynthesis from 4-dione, while its
ability of 5α-DHT inactivation to 3α-diol is quite lower 59
. As known, about 50% of Testo
in men is produced by the Leydig cells of the testis, whereas the rest of Testo is produced
from the circulating 4-dione in peripheral tissues, in which 3α-HSD2 is a typical enzyme
involved in this process called intracrinology 5; 7
. In human prostate, both 3α-HSD2 and 3β-
HSD1 are highly expressed in its basal epithelial cells, and androgen receptor (AR) is
highly expressed in its luminal cells. DHEA can be converted into 4-dione by 3β-HSD1,
and then 4-dione can be catalyzed into Testo by 3α-HSD2 in basal epithelial cells. Next,
Testo is transformed into 5α-DHT by type 2 5α-reductase in both basal and luminal cells of
prostate. The most potent androgen 5α-DHT is binding to AR in luminal cells, in which
prostate cancer is developed 5; 60
. In female ovary, 3α-HSD2 is involved in the
transformation of 4-dione to Testo in the theca cells of ovary 61
. Subsequently, 4-dione and
Testo are transferred into the granulosa cells of ovary, in which they can be aromatized into
estrogens 5; 61
. In addition, 3α-HSD2 also shows 20α-HSD activity to inactivate
progesterone, which can protect the theca cells from progesterone that is produced by the
granulosa cells 61
. The expression of 3α-HSD2 can be detected in the epithelial cells of
normal and malignant breast tissue specimens from women. However, breast cancer
specimens possess significant higher expression of 3α-HSD2 than that of normal breast
tissue, and the patients with 3α-HSD2 overexpression show worse prognosis than other
patients 62; 63
. To date, a few crystal structures of human 3α-HSD2 in complex with
different substrates and inhibitors have been reported, which demonstrates the flexibility of
its substrate binding site 64; 65; 66; 67
.
Human 3α-HSD3 (AKR1C2) is one of the major research topics in this thesis, and will be
introduced in more details in the subsequent sections.
Human 3α-HSD4 (also named 20α-HSD or AKR1C1) is found in uterus, ovary and
placenta 27; 68; 69
. This enzyme is mainly responsible for the inactivation of progesterone to
yield 20α-hydroxyprogesterone (20α-OHProg) in the presence of NADPH. By controlling
progesterone levels in vivo, 3α-HSD4 is closely involved in endometrial development and
pregnancy maintenance, as well as neuronal function 70; 71
. Selective loss of 3α-HSD4 is
9
found in breast cancer samples and cell lines (T47D and MCF7), and the suppression of 3α-
HSD4 expression by specific siRNA shows an increased progesterone level in MCF10A
cells and a decreased growth of T47D cells 72
. In addition, the crystal structure of 3α-HSD4
in complex with 20α-OHProg has been reported 54
.
1.4 HUMAN 3ΑLPHA-HSD3
1.4.1 The biological functions of human 3α-HSD3
Human 3α-HSD3 (AKR1C2) is found in liver, brain, prostate, testis and adrenal 27; 50
. It
shares a high protein sequence identity of 97.8% with human 3α-HSD4 (20α-HSD) 73
. Only
seven residues are different between 3α-HSD3 and 3α-HSD4. These two enzymes show
significant difference in specificity of steroidal substrates 74
. In vitro, 3α-HSD3 can oxidize
3α-diol to 5α-DHT in the presence of NAD+. However, it acts as a reductase to degrade 5α-
DHT in prostate cells 75; 76
. As known, 5α-DHT is the most potent androgen 77
. The
inactivation of 5α-DHT by 3α-HSD3 can prevent the activation of androgen receptor 29
. A
decreased expression of 3α-HSD3 in prostate cancer was reported by Qing Ji et al., and
they also reported that 5α-DHT concentrations were remarkably higher in prostate tumor
compared with benign tissue, which could be speculated that the loss of 3α-HSD3 in
prostate cancer cells increased 5α-DHT dependent cell growth 76; 78
. However, another
research group reported that, among four types of human 3α-HSDs, 3α-HSD3 was the
major form that was overexpressed in patients with prostate cancer, and its overexpression
was associated with prostate cancer progression 79
. In breast cancer cells, the expression
levels of 3α-HSD3 and 3α-HSD4 are reduced as compared with normal tissue cells 72; 80
.
Human 3α-HSD3 is also known as the bile acid binding protein and can be inhibited by bile
acids such as ursodeoxycholate 81; 82
. Human 3α-HSD3 exhibits a remarkable activity to
reduce 5β-pregnanes and 5α-pregnanes 71
. In human brain, through the production of
neurosteroid allopregnanolone, 3α-HSD3 also has an ability to regulate the γ-aminobutyric
acid type A (GABAA) receptor, which can lead to anesthetic and anxiolytic effects 48; 83
. In
addition, 3α-HSD3 plays a role in the basal and glucocorticoid-induced 5α-DHT
inactivation in human preadipocytes 84
. In the pathogenesis of female hirsutism, a reduced
10
expression of 3α-HSD3 of hirsute women is found, which can elevate 5α-DHT level in
their tissue 85
.
Figure 1.3 The overall structure of human 3α-HSD3 with cofactors and steroids
The reported structures show that there are two monomers in one crystal asymmetric unit.
Monomer A is colored in magenta. Monomer B is colored in cyan. Atoms are colored as
follows. Green, carbon atoms of steroids (Testo) and cofactors (NADP+); blue, nitrogen;
red, oxygen; orange, phosphorus.
1.4.2 The crystal structures of human 3α-HSD3
There are three crystal structures of human 3α-HSD3 in complex with Testo/acetate,
ursodeoxycholate and citrate/acetate, respectively, are reported 52; 53; 86
. Interestingly, the
11
high resolution structure of the 3α-HSD3·NADP+·Testo/acetate complex was obtained by
co-crystallization with 4-dione. During the crystallization process, the C17 carbonyl group
of 4-dione was firstly reduced by the enzyme to produce Testo, which means that human
3α-HSD3 also possesses certain 17β-HSD activity. It is noteworthy that Testo is released
from the steroid binding site after reduction and reoriented itself with the C3 carbonyl
group pointing inside of the enzyme cavity 52
. Although 3α-HSD3 is a monomer in
solution, there are two enzyme molecules in the crystal asymmetric unit (Figure 1.3).
Moreover, an acetate molecule is located between Testo and the nicotinamide ring of the
cofactor, which is introduced from the crystallization condition. This acetate molecule is
stably binding in the catalytic site and its ketone group forms two hydrogen bonds with the
side chains of Tyr55 and His117, which mimics the C3 carbonyl group of Testo in the rat
3α-HSD3 complex 51
. Obviously, the acetate can remarkably distort the orientation of Testo
in the enzyme cavity. Thus, an adjusted crystallization condition without acetate is used to
obtain a new crystal of 3α-HSD3 in complex with 4-dione. This work is reported in chapter
3 of this thesis.
In the 3α-HSD3·NADP+·ursodeoxycholate complex, the carboxylate group of
ursodeoxycholate is binding toward the catalytic site of the enzyme, which is located at the
similar position of the acetate molecule in the Testo/acetate complex and forms hydrogen
bonds with Tyr55 and His117 53
. An overlay of these two structures shows that although
ursodeoxycholate and Testo are oriented upside down in the cavity, their C18 and C19
methyl group are pointing toward the side chains of Val54 and Tyr55 and their α-faces of
ligands are stacking with the indole ring of Trp227. Meanwhile, the side chains of Val128,
Leu306 and Leu308 in two complexes are flipping about 180°, which demonstrates that the
steroid binding site possesses a considerable flexibility.
To understand the flexibility of the steroid binding site, the 3α-
HSD3·NADP+·citrate/acetate complex was reported
86. The citrate and acetate molecules,
which were introduced from the crystallization step, were found deeply embedded in the
steroid binding pocket. The acetate molecule is located at the same position as it in the
Testo/acetate complex, whereas the volume of its steroid binding pocket is reduced
considerably compared with that of the Testo/acetate complex. In addition, the replacement
12
of two residues Arg301 and Arg304, which are adjacent to the steroid binding pocket,
remarkably influences the 3α-HSD activity of the enzyme. These observations support an
“induced-fit” mechanism that the steroid binding pocket undergoes considerable
conformational changes to create a suitable binding site for its substrates.
Figure 1.4 The detailed interactions between 3α-HSD3 and NADP+
Atoms are colored as follows. Green, cofactor (NADP+) carbon; cyan, protein carbon; blue,
nitrogen; red, oxygen; orange, phosphorus. Hydrogen bonds are shown by black dashed
lines.
1.4.3 The conserved NADP+ binding site
The cofactor is clearly defined in the crystal structures, and is maintained in an extended
conformation across the (α/β)8-barrel (Figure 1.4). Its nicotinamide ring is located at the
center of the barrel, which is stacking with the side chain of Tyr216 and forms the bottom
of the steroid binding pocket. Meanwhile, the side chains of Ser166, Asn167 and Gln190
form hydrogen bonds with the nicotinamide ring of the cofactor. The ribose group of the
13
cofactor also forms hydrogen bonds with Thr23, Tyr24 and Asp50 to stabilize itself. The
pyrophosphate portion is stabilized by a numbers of hydrogen bonds with the back-bone
nitrogen atoms of Ser217, Leu219, Ser221, His222, Lys270 and the side chain of Ser217.
In addition, the 2’-phosphate group of the adenosine moiety is stabilized by salt bridges or
hydrogen bonds with Lys270, Ser271, Tyr272 and Arg276. Human 3α-HSD3 lacks a so-
called “safety belt” to firmly catch the cofactor, which is found in aldose reductase
subfamily and is also absent in rat 3α-HSD3 and human 20α-HSD 51; 54; 87; 88
. Interestingly,
even no cofactor is introduced during the protein purification and crystallization process,
NADP+ can be found in the crystal structures of the enzyme. This suggests that cofactors
coming from the E.coli cells are used in 3α-HSD3 catalysis 52; 86
.
Figure 1.5 The detailed interactions in the steroid binding site of 3α-HSD3
(A) The steroid binding site of the 3α-HSD3·NADP+·Testo complex; (B) The steroid
binding site of the 3α-HSD3·NADP+·ursodeoxycholate (urso) complex. Atoms are colored
as follows. Green, carbon atoms of cofactors and steroids; magenta, protein carbon in
figure 1.5 (A); cyan, protein carbon in figure 1.5 (B); blue, nitrogen; red, oxygen; orange,
phosphorus. Hydrogen bonds are shown by black dashed lines.
14
Figure 1.6 Proposed catalytic mechanism of 3α-HSDs
For the reduction, Tyr55 (Y55) acting as a general acid by donating its proton to the
acceptor carbonyl of the steroid, facilitated by protonation of the tyrosyl hydroxyl group by
the imidazole ring of His117 (H117). For the oxidation, Tyr55 (Y55) acting as a general
base by using its phenolate anion to abstract a proton from steroid alcohol, facilitated by
deprotonation of the tyrosyl hydroxyl group by the ε-amino group of Lys84 (K84). (This
figure is from Schlegel B. P. et al., Biochemistry, 1998.)
1.4.4 The steroid binding site
The steroid binding site of human 3α-HSD3 is formed by loop A (residues 117-143), loop
B (residues 217-238), loop C (residues 299-323), and two short loops (residues 23-32 and
51-57), which also includes the nicotinamide ring of the cofactor that lying at the bottom of
the cavity. In particular, 12 residues mainly located on these loops clearly define the
15
boundary of the cavity, which are Tyr24, Val54, Tyr55, Trp86, His117, Val128, Ile129,
His222, Trp227, Leu306, Leu308 and Phe311 52; 53
(Figure 1.5). In the 3α-
HSD3·NADP+·ursodeoxycholate complex, there is an additional hydrogen bonds between
the 7β-hydroxyl group of ursodeoxycholate and the side chain of Tyr24, which leads to an
increase of the binding affinity for this bile acid 53
.
1.4.5 Catalytic mechanism
The catalytic mechanism of human 3α-HSD3 follows an ordered bi-bi mechanism, in which
the cofactor binds firstly and then the steroid binds to the enzyme, after the reaction, the
steroid product is released from the enzyme before the release of the cofactor 89
. Based on
the rat 3α-HSD structure, a general mechanism is suggested for the oxidoreduction
catalyzed by 3α-HSDs 51; 90; 91
(Figure 1.6). In this mechanism, the C4 atom of the
nicotinamide ring is located neighboring to four residues of Asp50, Tyr55, Lys84 and
His117. These four residues are conserved in 3α-HSDs and form a catalytic tetrad. For the
reduction, a hydride (a proton with two electrons) from the C4 position of the nicotinamide
ring is directly transferred to the carbonyl group of the steroid, in which Tyr55 acts as a
general acid to donate its proton to the carbonyl group of the steroid. For the oxidation,
Tyr55 acts as a general base to extract a proton from the hydroxyl group of the steroid,
which can assist a hydride to transfer back to the cofactor. The acid-base ability of Tyr55 is
fulfilled by forming hydrogen-bond chains with Lys84 and His117 under different pH
conditions.
1.4.6 Kinetic features of human 3α-HSD3
The previous result shows that the C17 carbonyl group of 4-dione can be reduced by human
3α-HSD3 to output Testo during the crystallization process 52
. Thus, further kinetic studies
were performed to compare the 3α-HSD activity and its 17β-HSD activity of human 3α-
HSD3. The reported results show that, for the 3α-reduction of 5α-DHT, the steady-state
kinetic parameters are Km = 1.1 μM, kcat = 1.5 min-1
and kcat/Km = 1.3 min-1
μM-1
. For the
17β-HSD reduction of 4-dione, these parameters are Km = 1.38 μM, kcat = 0.067 min-1
and
kcat/Km = 0.049 min-1
μM-1
52
. The kinetic results clearly show that the 3α-HSD activity is
more favored by the enzyme than its 17β-HSD activity. In addition, a lower kcat/Km value
16
(Km = 2.90 μM, kcat = 1.98 min-1
and kcat/Km = 0.68 min-1
μM-1
) for the 3α-reduction of 5α-
DHT by the enzyme is reported from the group of Penning 92
. Besides, they also
demonstrate that four types of human 3α-HSDs convert 5α-DHT not only to 3α-diol but
also to 3β-diol, and the ratio of 3α-HSD/3β-HSD activity varies remarkably among human
3α-HSDs. In particular, human 3α-HSD3 predominantly acts as a 3α-HSD, whereas 3α-
HSD4 plays a major role of 3β-HSD 58
.
1.5 HUMAN NUCLEAR RECEPTORS
The nuclear receptors (NRs) are an evolutionarily conserved superfamily of transcription
factors (TFs) that are responsible for binding physiological hormones and other signaling
molecules 93; 94
. Activated by the binding of ligands, nuclear receptors can directly interact
with the promoter or enhancer of specific genes to initialize up-regulation or down-
regulation of transcriptions. As a consequence, nuclear receptors play important roles in
numerous physiological functions such as embryonic development, metabolic homeostasis,
salt balance and reproductive health 95; 96
. Moreover, many genes regulated by nuclear
receptors control key pathways involved in various diseases from cancers to metabolic
diseases. About 13% of U.S. FDA approved drugs use nuclear receptors as their drug
targets 97
.
1.6 HUMAN ESTROGEN RECEPTOR ALPHA
Estrogen receptor (ER) is a well-defined member of NRs superfamily. Through binding to
17β-estradiol (E2), ER controls sexual development and reproductive functions, and also
affects bone, cardiovascular, immune and central nervous systems 98
. In mammals, ERα
and ERβ are the two reported ER subtypes. ERα was firstly cloned from MCF7 human
breast cancer cell in 1980s. Human ERα gene (ESR1) is located on chromosome 6 99; 100
. In
the following ten years, human ERβ gene (ESR2) was cloned out. ESR2 is located on
chromosome 14 101; 102
. ESR1 and ESR2 both have eight exons separated by 7 introns and
other splice isoforms of both ERα and ERβ have deletion of exon3, exon4, or both 103
. ERα
and ERβ share common structural domains. In the presence of 17β-estradiol, ERα
stimulates MCF7 cell proliferation, whereas ERβ has a role to attenuate this effect 104
.
17
Figure 1.7 Structural organization of ERα
(A) ERα contains five structural regions: the N-terminal region, the DNA binding domain
(DBD), the hinge region, the ligand binding domain (LBD) and the C-terminal region. (B)
The 3D model of ERα. (Figure 1.7 (B) is from www.rcsb.org/pdb/101/motm.do?momID=45)
Similar to all the members of NRs, ERα contains five structural regions: the N-terminal
region (A/B region), the DNA binding domain (DBD or C region), the hinge region (D
region), the ligand binding domain (LBD or E region) and the C-terminal region (F region)
(Figure 1.7). The N-terminal region (residues 1-180) contains the activation function region
1 (AF-1), which modulates transcriptional activation independent of the presence of 17β-
estradiol and provides phosphorylation sites or interacts with other regulatory proteins 103
.
To be noticed, this domain is intrinsically disordered and involved in transient protein-
protein interactions, which is a common feature in NRs and certain transcription factors
18
such as p53 105; 106; 107
. The DNA binding domain (residues 181-263) is highly conserved in
NRs and contains two zinc-finger motifs with each zinc ion chelated with four conserved
cysteines 108; 109
. Two ERα DBDs form a homodimer directly binding to the estrogen
response elements (EREs) in specific promoters or enhancers. Typically, ERα EREs is
composed of two half-sites separated by 3 base pairs to form a palindrome segment such as
5’-AGGTCA-nnn-TGACCT-3’ 110
. The ligand binding domain (residues 303-552) is a
globular domain formed by 12 α-helices and the ligand binding pocket lies in the space
between helix3 and helix11. The ligand recognition is mainly based on a combination of
hydrophobic interactions and specific hydrogen bonding networks. ERα LBD contains a
ligand-dependent activation function region 2 (AF-2), which includes helix12 and is
responsible for the recruitment of coactivator proteins 111; 112; 113
. The hinge region (residues
264-302) between DBD and LBD contains the nuclear localization sequence (NLS) and the
structural information about this region is still not clear 103
. The C-terminal region (residues
553-595) is known to impact ligands binding and regulates LBD interaction with
coregulators 114
.
17β-estradiol is a small hydrophobic ligand, which can diffuse through the cell membrane
and bind to unliganded ERα located in cytoplasm. The liganded ERα dissociates from heat
shock proteins to form the homodimer and then translocates from the cytoplasm into
nucleus 115
. After ERα DBD binding to EREs of specific genes, the liganded ERα LBDs
interact with certain coregulators to up or down regulate genes transcription. The
coregulators including coactivators and corepressors using their Leu-X-X-Leu-Leu
(LXXLL) motif bind to the AF2 region of LBD in the presence of a ligand 116
. A well-
characterized family of coactivators is p160, which consists of three members: steroid
receptor coactivators 1 (SRC-1, also named NCoA1), SRC-2 (also named NCoA2 or GRIP-
1) and SRC-3 (also named AIB1). All three SRCs have the ability to recruit CREB-binding
protein (CBP) and its homolog p300. CBP and p-300 possess histone acetyltransferase
(HAT) activity, which promotes chromatin more accessible to form the RNA Pol II
transcription complex 103; 117; 118
. Corepressors including nuclear receptor corepressor
(NcoR) and silencing mediator for retinoid and thyroid hormone receptor (SMRT)
negatively regulate gene expression. Binding to ERα LBD in the appropriate ligand,
19
corepressors recruit proteins containing histone deacetylase (HDAC) activity, which
repress transcription by maintaining a condensed chromatin 103; 119; 120
.
Figure 1.8 ERα in complex with ligands and coregulators
ERα agonists such as 17β-estradiol cause a conformational change in the LBD, particularly
in H12 (red), which supports the formation of binding surface for the coactivator (SRC-1,
shown in purple). ERα antagonists such as raloxifene induce alternate conformations in the
LBD in which H12 is shifted away from its agonist conformation, which results in a larger
crevice that can accommodate a corepressor (SMRT, shown in blue). (Figure 1.8 is from
Huang P. et al., Annual Review of Physiology, 2010.)
ERα LBDs bind a variety of ligands with significant structural and functional diversity
(Figure 1.8). Some ligands act as agonists, while other ligands act as antagonists. The
agonists bind to LBD similar to the natural ligand 17β-estradiol such as the synthetic ligand
diethylstilbestrol (DES). Agonist binding stabilizes helix12 to form a lid on the ligand
binding pocket and thereby generates a competent AF2 region to recruit coactivator 111; 113
.
In contrast, antagonists such as Raloxifene and 4-hydroxytamoxifen (OHT) have extended
side chains to displace helix12, which prevents helix12 forming a functional AF2 region.
However, unlike coactivators, corepressors can bind to LBDs in the presence of antagonists
94; 121. In addition, SERMs (selective estrogen receptor modulators) act as agonists in
certain tissues, while they act as antagonists in other tissues. The ideal SERM should be an
20
ER antagonist in breast, and an ER agonist in bone, brain or other selected tissues.
Tamoxifen is the first well-characterized SERM and acts as antagonist in breast, but
tamoxifen results in an increase of endometrial cancer 122
. A possible explanation is that
tamoxifene is an antagonist in breast cancer cells for its recruitment of corepressors, while
tamoxifene is an agonist in endometrial cells for its recruitment of coactivators 123
.
Raloxifene is a second-generation SERM. However, it has similar function as tamoxifene
in breast cancer cells but has no negative effects on endometrial cell growth 117
. The
function of SERM suggests that the recruitment of different coregulators determines the
function of ER in different tissues.
Scientist’s interest for the structural studies of NRs has been alive for more than twenty
years. Due to difficulties in protein expression, purification and crystallization of the full-
length NRs, NRs DBDs and LBDs have been studied separately. The reported structures of
NRs DBDs and LBDs show the detailed structural-functional relationship and greatly
promote the rational drug design against these valuable targets 103; 124; 125; 126; 127; 128; 129; 130
.
In particular, the solution and crystal structures of ERα DBD with or without EREs, as well
as the crystal structures of ERα LBD in complex with agonists, antagonists and coactivator
are reported 108; 109; 110; 111; 112; 113
. However, in recent years, a growing number of studies
show that NRs DBDs and LBDs exert their functions as a whole. In 2008, Rastinejad group
reported the first full-length structure of PPARγ-RXRα heterodimer bound to DNA target,
ligand and coactivator peptide, which indicates that PPARγ LBD cooperates with both
heterodimer DBDs to enhance their binding to DNA response elements 131
. Moreover,
thyroid receptor showed higher binding affinity to its DNA response elements than its
isolated DBD alone 132
. Recently, Griffin and coworkers reported that NRs DBD binding to
DNA or its LBD binding to agonist is bi-directionally regulated by DBD and LBD 133
. In
addition, Chambon and coworkers reported that when glucocorticoid receptor (GR) bound
with “negative” DNA response elements, even GR bound with an agonist will still induce
direct transcriptional repression, which implies that DNA response elements is also a player
to regulate gene transcription 134
.
Therefore, the mechanism of bi-directional regulation between NRs DBDs bound with
DNA response elements and LBDs bound with ligands should be investigated further. This
21
is a driving force for us to purify ERα DBD-LBD and try to obtain the crystal of this
important hormone receptor in complex with its EREs.
1.7 THE TOPICS OF THE RESEARCH PROJECTS
The major topics discussed in this thesis are as following:
(1) Human 3α-HSD3 shares 97.8% protein sequence identity with 20α-HSD and only one
amino acid difference (residue 54) is located on their steroid binding pocket. Does residue
54 play a dominant role to dictate the substrate specificity for these two enzymes? How
does the structural difference caused by residue 54 play its role for the steroid
discrimination? By combining the mutagenesis, kinetics and X-ray crystallography study,
we aim to answer these questions.
(2) Androgen 5α-DHT has been shown to prevent breast cancer cells growth and human
3α-HSD3 is characterized by its major ability to inactivate 5α-DHT. So, what is the
concrete interaction between 5α-DHT and 3α-HSD3? Does 3α-HSD3 play an important
role in breast cancer cells as it does in prostate cancer cells? By combining the X-ray
crystallography and the functional studies in the cellular level, we try to give certain
answers.
Besides, two topics related to human ERα are as following:
(1) Recently, a number of studies have showed that nuclear receptor DBDs and LBDs exert
their functions as a whole. However, due to difficulties in protein expression, purification
and crystallization, the full-length ERα structure remains unfulfilled. Here, we want to
establish an expression and purification protocol of ERα DBD-LBD, and try to crystallize
ERα DBD-LBD in complex with estrogen response elements.
(2) Several methods have been developed to purify ERα LBD, such as carboxymethylation
or mutation of reactive cysteine residues. Here, we develop a simple and efficient
purification method of ERα LBD by using a combination of detergents.
22
23
CHAPTER 2 STRUCTURE-FUNCTION STUDY OF HUMAN 3-
ALPHA HYDROXYSTEROID DEHYDROGENASE TYPE 3 (3ΑLPHA-
HSD3) V54L MUTATION
24
2.0 PREFACE
Human 3-alpha hydroxysteroid dehydrogenase type 3 (3α-HSD3) has an essential role in
the inactivation of 5α-dihydrotestosterone (5α-DHT), while human 20-alpha
hydroxysteroid dehydrogenase (20α-HSD) is responsible for the inactivation of
progesterone. However, there is only one amino acid difference (residue 54) between the
steroid binding pockets of 3α-HSD3 and 20α-HSD. Does residue 54 play a dominant role to
dictate the substrate specificity for these two enzymes? How does the structural difference
caused by residue 54 play its role for steroid discrimination? By combining mutagenesis,
kinetics and X-ray crystallography study, we want to find the answers for these questions.
This chapter includes one paper: Human 3-alpha hydroxysteroid dehydrogenase type 3 (3α-
HSD3): the V54L mutation restricting the steroid alternative binding and enhancing the
20α-HSD activity. In this paper, I carried out the experimental studies, solved the crystal
structures and wrote the manuscript. Dr. Dao-Wei Zhu guided the protein purification. Dr.
Xiao-Jian Hu checked the solved crystal structures. Dr. Ming Zhou guided enzyme kinetic
studies. Dr. Sheng-Xiang Lin and I designed the study.
25
Human 3-alpha hydroxysteroid dehydrogenase type 3 (3α-HSD3): the V54L mutation
restricting the steroid alternative binding and enhancing the 20α-HSD activity
Bo Zhang 1, 2
, Dao-Wei Zhu 1, Xiao-Jian Hu
3, Ming Zhou
1, Peng Shang
2, Sheng-Xiang
Lin 1, §
1 Laboratory of Molecular Endocrinology and Oncology, Centre Hospitalier Universitaire
(CHU) de Quebec Research Center (CHUL) and Laval University, Québec City, Québec,
G1V4G2, Canada
2 Key Laboratory for Space Bioscience & Biotechnology, Institute of Special
Environmental Biophysics, School of Life Sciences, Northwestern Polytechnical University,
Xi’an, P. R. China, 710072
3 School of Life Sciences, Fudan University, Shanghai, P.R. China, 200433
§ Corresponding Author: S.-X. Lin, CHUL Research Center, 2705 Boul. Laurier, Québec
City, QC, G1V4G2, Canada; Tel.: +1 418 654 2296
E-mail: [email protected]
Shortened title: Structure-function study of human 3α-HSD3 V54L mutation
26
2.1 ABSTRACT
Human 3-alpha hydroxysteroid dehydrogenase type 3 (3α-HSD3) has an essential role in
the inactivation of 5α-dihydrotestosterone (5α-DHT). Notably, human 3α-HSD3 shares
97.8% sequence identity with human 20-alpha hydroxysteroid dehydrogenase (20α-HSD)
and there is only one amino acid difference (residue 54) that is located in their steroid
binding pockets. However, 20α-HSD displays a distinctive ability in transforming
progesterone to 20α-hydroxy-progesterone (20α-OHProg). In this study, to understand the
role of residue 54 in the steroid binding and discrimination, the V54L mutation in human
3α-HSD3 has been created. We have solved two crystal structures of the 3α-
HSD3·NADP+·Progesterone complex and the 3α-HSD3 V54L·NADP
+·progesterone
complex. Interestingly, progesterone adopts two different binding modes to form
complexes within the wild type enzyme, with one binding mode similar to the orientation
of a bile acid (ursodeoxycholate) in the reported ternary complex of human 3α-
HSD3·NADP+·ursodeoxycholate and the other binding mode resembling the orientation of
20α-OHProg in the ternary complex of human 20α-HSD·NADP+·20α-OHProg. However,
the V54L mutation directly restricts the steroid binding modes to a unique one, which
resembles the orientation of 20α-OHProg within human 20α-HSD. Furthermore, the kinetic
study has been carried out. The results show that the V54L mutation significantly decreases
the 3α-HSD activity for the reduction of 5α-DHT, while this mutation enhances the 20α-
HSD activity to convert progesterone.
Keywords: 3-alpha hydroxysteroid dehydrogenase, AKR1C2, 20α-HSD, mutation, kinetics,
crystal structure
Protein data bank accession codes: 4L1W and 4L1X
27
2.2 INTRODUCTION
Human 3-alpha hydroxysteroid dehydrogenases (3α-HSDs) belong to the aldo-keto
reductase (AKR) superfamily and possess 3-keto-, 17-keto-, and 20-ketosteroid reductase
activities to catalyze the inactivation of androgens, estrogens, progestins, and bile acid
precursors 1; 2; 3
. In human, four isoenzymes of 3α-HSDs share at least 81% sequence
identity and show differential tissue distributions 4; 5; 6
. These enzymes are soluble
monomeric proteins and they use NADPH as their cofactor 5. According to the
nomenclature of AKR family, human 3α-HSD types 1, 2, 3 and 4 are named AKR 1C4,
1C3, 1C2 and 1C1, respectively. Human 3α-HSDs have no significant sequence similarity
with the short-chain dehydrogenase/reductase superfamily (SDR) such as 17β-HSDs and
11β-HSD 7; 8; 9; 10
.
Human 3α-HSD3 plays a major role in the reduction of 5α-DHT to 5α-androstane-3α,17β-
diol (3α-diol), which prevents the binding and activation of androgen receptor from
overflowing androgen 6; 11
. As known, 5α-DHT is the most potent androgen and excess of
5α-DHT has been associated with the development of benign prostatic hyperplasia and
prostate cancer in human 12
. Human 3α-HSD4 also named 20α-HSD (hereafter 20α-HSD is
used to represent this enzyme) transforms progesterone into 20α-OHProg in ovary, uterus
and placenta 5; 13; 14
. Human 20α-HSD shares 97.8% sequence identity with 3α-HSD3 and
there are only seven amino acids differences between two enzymes 15
. Human 3α-HSD2
(also recognized as 17β-HSD5) exhibits much higher ability in reducing 4-androstene-3,17-
dione (4-dione) to testosterone (Testo) than its ability in transforming 5α-DHT to 3α-diol 16
.
In mammary gland, 3α-HSD2 can also catalyze estrone to 17β-estradiol and progesterone
to 20α-OHProg 5. Human 3α-HSD2 and 3α-HSD3 are found to be highly expressed in
human prostate 5; 17
. Human 3α-HSD1 is a liver specific 3α-HSD, which plays a role of
inactivation 3-keto steroids in liver 5; 6
.
The reported structure of 3α-HSD3·NADP+·Testo/acetate complex shows that the enzyme
adopts an (α/β)8-barrel motif. The steroid binding pocket, which is mainly formed by loop
A, B and C, locates at the C-terminal end of the barrel 18
. Besides, the 3α-
HSD3·NADP+·ursodeoxycholate complex and the 3α-HSD3·NADP
+·citrate·acetate
28
complex reveal that the steroid binding pocket of the enzyme possesses remarkable
flexibility to bind different substrates 19; 20
. A general catalytic mechanism shows that a
hydride is directly transferred from the C4 position of the cofactor to the carbonyl group of
substrate and the enzyme acts as the proton donor simultaneously 21
.
Particularly, there is only one amino acid difference (residue 54) between the steroid
binding pockets of human 3α-HSD3 and 20α-HSD. Based on the kinetic study of certain
steroids or substrates in human liver, the earlier research showed that the mutation of
human 20α-HSD Leu54-to-Val54 produced an enzyme that possessing the similar
characteristic as 3α-HSD3 22
. However, the detailed spatial change caused by residue 54 in
the steroid binding pockets of both enzymes awaits a comparative structural study to
acquire better comprehension on the structure-function relationship. In addition, a
comparative kinetic study for the reduction of 5α-DHT and progesterone by human 3α-
HSD or 20α-HSD, and the corresponding residue 54 mutant has not been completely
investigated.
Here, we report the crystal structures of the 3α-HSD3·NADP+·progesterone complex and
the 3α-HSD3 V54L·NADP+·progesterone complex. It can be found that progesterone in the
wild type enzyme possesses two different binding modes. However, only one binding mode
of the steroid can be observed in the mutant enzyme. Furthermore, the kinetic study shows
that the V54L mutation in human 3α-HSD3 remarkably reduces the 5α-DHT degradation
ability of the enzyme and enhances the 20α-HSD activity to reduce progesterone.
2.3 MATERIALS AND METHODS
2.3.1 Materials
DTT and β-octyl glucoside (β-OG) were purchased from Gold Biotechnology. Thrombin
was purchased from MP Biomedicals. Progesterone and 5α-DHT were purchased from
Steraloids. Diethyl ether, toluene, acetone and dichloromethane were purchased from
Fisher Scientific. Thin layer chromatography (TLC) plate was purchased from EMD
Millipore. NADPH, NADP+ and other chemicals were purchased from Sigma-Aldrich.
14C-
29
Progesterone (55 mCi/mmol) was purchased from American Radiolabeled Chemicals and
14C-5α-DHT (53.5 mCi/mmol) was purchased from PerkinElmer Life Sciences.
2.3.2 Site-directed mutagenesis
The pGEX vector encoding the wild type human 3α-HSD3 was used as a template for
conducting human 3α-HSD3 V54L site-directed mutagenesis. The mutation was performed
using QuikChange Lightning Kit (Agilent Technologies) with 5’-
CCATATTGATTCTGCACATTTATACAATAATGAGGAGC-3’ as forward primer and
verified by sequencing.
2.3.3 Protein expression and purification
The recombinant wild type human 3α-HSD3 with a glutathione S-transferase (GST) tag
was overexpressed in E. coli BL21(DE3)pLysS cells and purified by following a previously
described procedure 23
. In brief, the enzyme was firstly purified with a glutathione agarose
column in PBS buffer (pH 7.4) and the GST fusion tag was cut by thrombin overnight at
4°C. Another step of Q-sepharose column purification with a salt gradient using buffer A
(25 mM Tris-HCl (pH 7.4), 0.5 mM DTT, 0.06% β-octyl glucoside (β-OG), 1 mM EDTA,
10% Glycerol) and buffer B (buffer A with 500 mM NaCl) yields high purity enzyme. The
fractions of 3α-HSD3 were concentrated to 28-30 mg/ml in a 10 mM KH2PO4-K2HPO4
buffer (pH 7.0) containing 0.5 mM DTT, 0.06% β-OG, 1 mM EDTA, 1 mM NADP+ and
40 μM progesterone. The recombinant human 3α-HSD3 V54L was overexpressed and
purified as the wild type enzyme. Protein purity was checked by SDS-PAGE and protein
concentration was determined by Bradford assay. The concentrated 3α-
HSD3·NADP+·Progesterone or 3α-HSD3 V54L·NADP
+·progesterone was preserved at -
80°C for later crystallization.
2.3.4 Crystallization
Crystals were obtained by vapor diffusion method using both hanging drops and sitting
drops at room temperature. For both complex crystals, the reservoir solution contained 100
mM sodium cacodylate buffer (pH 6.0), 200 mM ammonium sulfate, 24-26% (w/v)
polyethylene glycol (PEG) 3350. Prior to crystallization, 40 mM progesterone stock in
30
ethanol was added into the 0.5 ml reservoir solution to reach the final 0.8 mM progesterone.
Crystals appeared in 3 days and reached to their final size in two weeks. The reservoir
solution containing 15% glycerol was used as a cryoprotectant for the flash-cooled crystals
in liquid nitrogen.
2.3.5 Data collection and structure determination
Diffraction data were collected from the Advanced Photon Source (APS) at Argonne
National Laboratory. Data images were recorded while the single crystal was rotated from 0°
to 180° by 1° steps. Data sets were indexed and integrated by iMosflm version 1.0.7 24
. The
space group for both complex crystals was P21 and the asymmetric unit for each crystal
contained two monomers. The 3α-HSD3·NADP+·progesterone and 3α-HSD3
V54L·NADP+·progesterone structures were solved by molecular replacement using Molrep
in CCP4 Program Suite 6.2.0 25; 26
. The subunit A of the 3α-HSD3·NADP+·Testo/acetate
structure omitting Testo and the solvent (Protein Data Bank code 1J96) was used as a
search model 18
. Multiple rounds of refinement and model building were performed using
the program Refmac in CCP4 27
and COOT 28
, respectively. Subsequently, NADP+ and
progesterone were fitted into the electron density map and refined. The geometry of the
final models was verified with the program PROCHECK in CCP4 29
.
2.3.6 Kinetic analysis of the wild type and the mutant 3α-HSD3
The enzyme for kinetic study was purified as described above. The only difference was that
the wild type and the mutant 3α-HSD3 were concentrated to 1 mg/ml in buffer A without
steroids and cofactors (NADPH and NADP+). The enzyme concentration was determined
by Bradford assay. Reduction reactions on 14
C-steroids were conducted. Each kinetic
reaction was performed at 37.0 ± 0.3°C in a volume of 1 ml 25 mM Tris-HCl buffer (pH
7.4) containing 10% Glycerol, 300-400 μM NADPH and 0.01 mg/ml of BSA. The reaction
was initiated by adding the enzyme to the reaction mixture. When 5α-DHT was used as
substrate, the wild type and the mutant enzyme were added to the reaction mixture to reach
to the final concentration of 0.2 μg/ml and 1.2 μg/ml, respectively. When progesterone was
used as substrate, the final concentrations of the wild type and the mutant enzyme were 1.0
μg/ml and 0.5 μg/ml, respectively. After different time intervals, the reactions were stopped
31
by the adding 3 volumes of diethyl ether. Following a typical TLC protocol previously
described 30
, steroids were separated and TLC plates were exposed and quantified by using
a Storm imaging system. Initial velocities were calculated by less than 10% steroids
consumption. At least duplicates of independent experiments were carried out for each Km
and kcat determination.
2.4 RESULTS
2.4.1 Overall structure of the wild type and the mutant 3α-HSD3
The crystal structures of two ternary complexes 3α-HSD3·NADP+·progesterone and 3α-
HSD3 V54L·NADP+·progesterone have been solved. Prior to crystallization, progesterone
was added into the 0.5 ml reservoir solution to reach the final 0.8 mM. This step can be
used to replace soaking progesterone into the crystal afterwards, which can saturate the
enzymes with excess steroids and avoid cracking the crystal during the soaking process.
Crystals of two ternary complexes 3α-HSD3·NADP+·progesterone and 3α-HSD3
V54L·NADP+·progesterone belonged to the monoclinic space group P21 and contained two
monomers (monomer A and B) in the asymmetric unit (Figure 2.1(A)). The 3α-
HSD3·NADP+·progesterone complex was refined at 2.2 Å with a crystallographic R-factor
of 14.6% and an R-free factor of 19.4%. The 3α-HSD3 V54L·NADP+·progesterone
complex was refined at 2.0 Å with an R-factor of 14.0% and an R-free factor of 18.3%.
Data collection and refinement statistics are shown in Table 2.1. The protein chains in both
refined models are highly similar to each other and to the previously reported structures of
human 3α-HSD3 in complex with Testo/acetate and ursodeoxycholate 18; 19
. The major
differences in these structures only exist in the regions around the steroid binding site.
2.4.2 Conserved NADP+ binding
The electron density map unambiguously defines the NADP+ stable binding to the enzyme,
which shows a highly similar conformation for NADP+ as described previously
18; 19. The
NADP+
phosphate group is well located between the two side chains of Lys270 and Arg276.
The π-π stacking between the NADP+ nicotinamide ring and the Tyr216 phenol group also
contributes to NADP+ stabilization. Besides, a number of hydrogen bonds and Van der
32
Waals interactions between NADP+ and the cofactor binding site have been revealed earlier
18; 19.
2.4.3 The ternary complex of human 3α-HSD3·NADP+·progesterone
The 3α-HSD3·NADP+·progesterone complex has been obtained by co-crystallization as
described in methods. The Fourier difference map clearly indicates that two progesterone
molecules are located in the steroid binding sites in monomer A and B. However,
progesterone in monomer A shows a lower average B-factors. In order to obtain
comparable B-factors, the occupancy of progesterone in monomer B is set to 0.8. As
observed in human 20α-HSD in complex with 20α-OHProg 31
, progesterone is positioned
with its O20 atom pointing toward the nicotinamide ring. In monomer A of human 3α-
HSD3, the β-face of progesterone interacts with the Trp227 side chain and its α-face
interacts mainly with Val54 and Val128. This allows the steroid C18 and C19 methyl
groups to point toward Trp227 (Figure 2.1(B)). While, in its monomer B, the two methyl
groups are pointing toward Tyr55 and the steroid α-face is in stacking with Trp227 side
chain (Figure 2.1(C)). Consequently, when monomer A and B are superimposed, two
steroids could not overlap each other and their orientations have an about 105° rotation
difference around the long axis of C10-C17 (Figure 2.1(D)). With this rotation, the distance
between the nicotinamide ring C4 atom and progesterone C20 atom is changed from 4.15 Å
in monomer A to 4.37 Å in monomer B. Meanwhile, the distance between the steroid O20
atom and His222 Nε atom is changed from 3.19 Å in monomer A to 5.46 Å in monomer B.
As known, the steroid binding site is mainly formed by loop A (residues 117-143), loop B
(residues 217-238), loop C (residues 299-323), and two short loops (residues 23-32 and 51-
57). When monomer A and B are superimposed, the RMSD value is 0.40 Å for 323 amino
acids Cα atoms. Meanwhile, the RMSD values are 1.09 Å, 0.46 Å and 0.23 Å for loop A,
loop B and loop C, respectively, which indicates that the back bone of loop A fluctuates
notably compared with loop B and loop C. Further inspection of the steroid binding site,
residues 126-141 in loop A exhibits a considerable displacement toward loop B. The
conformational changes of loop A drive the side chains of Val128, Ile129 moving closer to
the steroid, which may generate the forces to rotate progesterone in its binding site.
Moreover, the side chains of Leu54, Trp227, Leu306 and Leu308 reconcile their
33
conformations to accommodate the steroid. In addition, the crystal structure reveals that a
water molecule presents at the catalytic site and forms two hydrogen bonds with the side
chains of Tyr55 and His117, which exactly occupies the same position instead of the ketone
group from Testo, acetate or ursodeoxycholate in the reported ternary complexes 18; 19; 20; 32
.
In monomer B, this key water molecule can also participate in the stabilization of
progesterone through a hydrogen bond with the steroid O20 atom. In monomer A and B,
the orientations of the steroid C20 ketone groups as well as the distances between the C20
atoms and the nicotinamide ring C4 atoms are not suitably coordinated for the hydride
transfer, and such conformations represent the steroid binding modes before or after the
reaction.
2.4.4 The ternary complex of human 3α-HSD3 V54L·NADP+·progesterone
The 3α-HSD3 V54L·NADP+·progesterone structure shows high similarity to the ternary
complex of the wild type enzyme and the 20α-HSD ternary complex 31
. The electron
density map clearly defines that progesterone is situated in the steroid binding site, in which
the Leu54 side chain in the mutant enzyme is outstretching toward the steroid (Figure
2.2(A)). Consistent with the wild type enzyme, in the mutant enzyme, the temperature
factor for progesterone in monomer B is higher than that in monomer A. Therefore, the
occupancy of progesterone in monomer B is set to 0.8 to acquire a comparable B-factor.
However, when superimposing monomer A with B (Figure 2.2(B)), the orientations of two
steroids overlap each other quite well, which is different from the 3α-
HSD3·NADP+·progesterone structure. The β-faces of both steroids interact with the Trp227
indole group and their α-faces interact mainly with Leu54 and Val128. After superposition,
the RMSD value for 323 amino acids Cα atoms between monomer A and B is 0.35 Å. The
RMSD values for loop A, loop B and loop C are 0.85 Å, 0.34 Å and 0.18 Å, respectively.
Although loop A displays a movement to loop B and the side chains of Val128, Ile129 get
closer to the steroid at the same time, the conformation of progesterone seems be fixed in
its binding pocket and hardly any rotation can be observed. It is not difficult to understand
that the bulky side chain of Leu54 generates a steric hindrance to restrict the steroid
rotation. Even though the average B-factors for the wild type enzyme and the mutant
enzyme are quite similar (Table 2.1), the average B-factors for steroids in the mutant
34
enzyme (monomer A/monomer B) hold the relative lower B-factors (23.3/27.6 Å2) than
that in the wild type enzyme (37.7/34.4 Å2), indicating that the V54L mutation has a role in
the stabilization of progesterone. In addition, the side chains of Trp227, Leu306 display
slight movements and the side chain of Leu308 flips 90° around its Cβ. Besides, a water
molecule forms hydrogen bonds with Tyr55, His117 and situates at the catalytic site.
2.4.5 Kinetic study of the wild type and the mutant 3α-HSD3
To investigate how significantly the mutation of Val54 to Leu54 in human 3α-HSD3 alters
the enzyme activity and its steroid binding specificity, the relevant kinetic study were
carried out. Firstly, the wild type enzyme or the V54L mutant enzyme (the final
concentration of 1 μg/ml) was added into the reaction mixture to initiate the reaction, and
the reaction mixture contained 300 μM NADPH. When 5α-DHT or progesterone was used
as substrate at the concentration of 4 μM, after 10 minutes reaction at 37°C, the TLC was
performed. The result demonstrates that the V54L mutation remarkably reduces the 3α-
HSD reduction ability for 5α-DHT and enhances the 20α-HSD reduction activity for
progesterone (Figure 2.3). Furthermore, to obtain more detailed kinetic information, the
steady-state kinetic study was performed (Table 2.2). When 5α-DHT was used as substrate,
the specificity constant (kcat/Km) for the mutant enzyme was decreased to 17-fold. This
denotes that, compared with the wild type enzyme, the V54L mutation significantly reduces
the 3α-HSD3 specificity for 5α-DHT. When progesterone was used as substrate, the kcat/Km
value was increased to 4.4-fold and the mutant enzyme has gained a considerable 20α-HSD
activity.
2.5 DISCUSSION
In this study, it is interesting to show that progesterone can adopt two different binding
modes to form complexes with monomer A and B of the wild type 3α-HSD3 in a crystal
asymmetric unit, respectively. However, the V54L mutation in the enzyme directly restricts
the steroid binding modes to a unique one.
When monomer A and B in the 3α-HSD3·NADP+·progesterone complex are superimposed,
it can be clearly seen that, in monomer B, loop A has a major movement toward loop B and
35
progesterone (Figure 2.1(D)). This is mainly due to the different interacting environments
with the neighboring symmetric molecules for monomer A and B. Correspondingly, in
monomer B, the two hydrophobic residues Val128 and Ile129 in loop A are moving inside
the steroid binding pocket a little and their side chains make closer van der Waals contacts
with the A ring of the steroid. The side chain of Leu308 flips 180° around its Cβ atom and
the side chain of Leu306 owns alternative conformations. Meanwhile, progesterone
presents a 105° rotation around its C10-C17 axis. The interaction between His222 Nε atom
and the O20 atom of the steroid is within the range of hydrogen bond in monomer A. While
in monomer B, this interaction is greatly reduced and the side chain of His222 flips 180°
around its Cβ atom. The superposition shows that the steroid binding pocket of 3α-HSD3
possesses a considerable flexibility, which allows two different steroid binding modes for
progesterone. In addition, it has been proved that human 3α-HSD3 can bind with several
ligands such as citrate and ursodeoxycholate 19; 20
, which further validates the flexibility of
the steroid binding pocket.
In the 3α-HSD3 V54L·NADP+·progesterone complex, the overlay of monomer A and B
shows high similarity for the overall structure (Figure 2.2(B)). Although loop A in
monomer B also displays a shift toward loop B, the orientation of progesterone has not
been transformed. Obviously, Leu54 plays a key role to eliminate multiple orientations
which are allowed in the wild type enzyme. If progesterone in the mutant enzyme has a 105°
rotation like it does in the wild type enzyme, the C ring of the steroid will conflict with the
bulky side chain of Leu54. Therefore, despite the steroid binding pocket possessing
considerable flexibility, the V54L mutation significantly restricts the movement space of
the steroid. An overlay of both monomers A in the wild type and the mutant enzyme shows
progesterone has a minor shift toward Trp227 in the mutant enzyme and the indole ring of
Trp227 has an 11° rotation around its Cβ atom (Figure 2.4(A)). At the same time, the side
chain of Ile129 rotates about 103° around its Cγ atom and the side chain of Leu308 flips
about 180° around its Cβ atom, which represents the flexibility of this cavity. When the
V54L mutant complex and the 20α-HSD·NADP+·20α-OHProg complex are superimposed,
the plane of the steroid has a slight swing around the short axis of C13-C18. Meanwhile,
the side chains of Ile129, Trp227 and Leu308 possess subtle movements and the side chain
of Leu306 flips 180° around its Cβ atom (Figure 2.4(B)). Although six amino acids
36
difference between the 3α-HSD3 V54L mutant and 20α-HSD still remains, these residues
do not disturb the overall arrangement of the main chains in both enzymes.
In human 3α-HSD3 and 20α-HSD, the indole rings of Trp227 adopt similar orientations to
stack with the plane of the steroid and have a crucial role to stabilize the orientation of the
steroid. However, compared with their homologous human steroid 5β-reductase (AKR1D1)
33, the indole ring of Trp227 (numbering according to 3α-HSD3) rotates about 125° toward
the side chain of Val228. It can be seen that the steroid and the indole ring of Trp227 in
AKR1D1 adjust their orientations to satisfy the bulky side chains of Ile128 and Tyr129 (3α-
HSD3 numbering) in loop A stretching into the steroid binding pocket. Besides, the less
bulky side chains of Ser222 and Val306 (3α-HSD3 numbering) in loop B can accommodate
the reorientation of Trp227.
An overlay shows the orientation of ursodeoxycholate in the reported 3α-
HSD3·NADP+·ursodeoxycholate complex is quite identical to that of progesterone in
monomer B of the 3α-HSD3·NADP+·progesterone complex, in which both C18 methyl
groups are pointing toward Tyr55 side chain (Figure 2.4(C)). However, compared with the
orientation of progesterone in the 3α-HSD3 V54L·NADP+·progesterone complex, the
orientation of ursodeoxycholate needs an about 105° rotation around its C10-C17 axis to
overlap with the plane of progesterone (Figure 2.4(D)). But this rotation is not allowed for
the reason that the carboxylate group of ursodeoxycholate will collide with the imidazole
ring of His222. Besides, the overlay shows that the distance between ursodeoxycholate C18
atom and Leu54 Cγ atom in the mutant enzyme is about 2.48 Å, which implies the bulky
side chain of Leu54 will obstruct the ursodeoxycholate binding by this orientation. Hence,
the orientation of ursodeoxycholate in the wild type 3α-HSD3 should be the unique one for
the reason that the less bulky side chain of Val54 is located in the steroid binding pocket.
As reported 19; 34
, human 3α-HSD3 is the only one that can bind ursodeoxycholate among
human 3α-HSDs. All the other three types of human 3α-HSDs have Leu54 residues at this
position.
Based on the docking simulation of 5α-DHT into human 3α-HSD3 and 20α-HSD, the
swinging mechanism has been proposed that the shorter side chain of Val54 in 3α-HSD3
prefers to produce 3α-diol, while the bulky side chain of Leu54 in 20α-HSD can generate a
37
swing of 5α-DHT to produce 3β-diol 35; 36
. From our structural results, superposition of the
wild type 3α-HSD3 and the V54L mutant demonstrates that the orientation of progesterone
in their monomer A does not show such kind of swing, while the orientation of the steroid
in their monomer B displays a 105° rotation. This rotation of the steroid orientation is
similar to the flipping mechanism that the plane of the steroid can flip around its long
molecular axis to bind in its cavity 37
.
To further understand the steroid discrimination by human 3α-HSD3 and its V54L mutant,
the kinetic study has been carried out. A single V54L mutation in 3α-HSD3 significantly
decreases its 3α-reductase activity and enhances its 20α-reductase activity. For 5α-DHT
reduction, the steady-state kinetic parameters for the wild type enzyme are Km = 2.18 μM,
kcat = 3.67 min-1
and kcat/Km = 1.68 min-1
μM-1
. When compared with the former results by
our group (Km = 1.1 μM, kcat = 1.5 min-1
and kcat/Km = 1.3 min-1
μM-1
), the kcat/Km values are
similar to each other 18
. The relevant result from the group of Penning (Km = 2.90 μM, kcat =
1.98 min-1
and kcat/Km = 0.68 min-1
μM-1
) shows a slight difference 38
. However, the kinetic
parameters for the V54L mutant (Km = 71.03 μM, kcat = 6.92 min-1
and kcat/Km = 0.10 min-1
μM-1
) clearly shows its 5α-DHT reduction specificity is significantly decreased. While for
progesterone reduction, the wild type enzyme exhibits a weak activity (Km = 0.84 μM, kcat =
0.21 min-1
and kcat/Km = 0.25 min-1
μM-1
), but the mutant enzyme shows a considerable
20α-reductase activity (Km = 2.13 μM, kcat = 2.35 min-1
and kcat/Km = 1.10 min-1
μM-1
). The
3α-HSD3 V54L mutant imitates human 20α-HSD and its enzyme activity is higher than the
reported human 20α-HSD activity for progesterone reduction by the group of Penning (Km
= 2.65 μM, kcat = 0.29 min-1
and kcat/Km = 0.11 min-1
μM-1
) and by the group of Bunce (Km =
4.20 μM, kcat = 1.77 min-1
and kcat/Km = 0.42 min-1
μM-1
) 5; 39
, and is similar to the reported
result by the group of Hara (Km = 1.30 μM, kcat = 1.50 min-1
and kcat/Km = 1.20 min-1
μM-1
)
40. The differences of the kinetic parameters may attribute to the different buffer systems
and temperatures used for the reactions. In addition, the kinetic study demonstrates that
17β-HSD1 also possesses certain 5α-DHT reduction activity (Km = 32.0 μM, kcat = 2.40
min-1
and kcat/Km = 0.08 min-1
μM-1
) 30
, but it is far less than the specificity constant (kcat/Km)
of the wild type 3α-HSD3 and is only comparable to that of the V54L mutant enzyme.
38
Besides the V54L mutation in human 3α-HSD3, a number of mutations targeting 3α-HSDs
have been carried out to evaluate the specific roles of different residues in the enzymes. A
previous experiment showed that two human 3α-HSD3 mutants (F46Y and L172Q) possess
reduced reductase activities 41
, and these mutants have been predicted to destabilize the
cofactor binding by the method of homology modeling 42
. Furthermore, formerly, an
attempt has been done to engineer mammalian (rat) 3α-HSD to 20α-HSD 43
. Both enzyme
share 67% protein sequence identity and six amino acid residues which locate in the steroid
binding site are different. However, even when all these six distinctive residues of rat 3α-
HSD were mutated to the relevant residues of rat 20α-HSD, the 20α-HSD activity was still
not available for the mutant enzyme. Compared with the results from human 3α-HSD3
V54L mutation, one reasonable explanation is that human 3α-HSD3 and 20α-HSD share
97.8% sequence identity, which is much higher than 67% sequence identity between the
two rat enzymes. The V54L mutation in human 3α-HSD3 can generate adequate
stereospecificity for the 20α-HSD activity. While for rat 3α-HSD, until loop A, B and C in
the steroid binding site are together replaced with the equivalent loops of 20α-HSD, the
similar task can be fulfilled 43
. In addition, the important mutagenesis experiment done by
Matsuura et al. demonstrated that the replacement of human 20α-HSD Leu54 with Val54
almost produced an enzyme possessing the similar property as 3α-HSD3 22
. Our kinetic
study is complementary to their mutagenesis and kinetic work.
In summary, the alternative binding modes of progesterone have been found in the wild
type 3α-HSD3, which indicates the steroid binding pocket possessing considerable
flexibility to accommodate different orientations of a steroid. However, the bulky side
chain of Leu54 in the mutant enzyme significantly confines the spatial movement of the
steroid in its cavity and thus only one orientation presents in its ternary structure. Moreover,
the kinetic study shows that the V54L mutation is enough to transform human 3α-HSD3 to
an enzyme with a competent 20α-HSD activity, whereas its 3α-HSD activity is significantly
decreased. This study gives us a hint that the alternative binding modes may also exist for
5α-DHT in human 3α-HSD3 and be utilized by the enzyme to output different products
such as 3α-diol and 3β-diol.
39
2.6 FUNDING SOURCES
This work was supported by the Canadian Institutes of Health Research (CIHR), with a
grant to Dr. Sheng-Xiang Lin and collaborators (MOP 97917). Use of the Advanced Photon
Source, an Office of Science User Facility operated for the U.S. Department of Energy
(DOE) Office of Science by Argonne National Laboratory, was supported by the U.S. DOE
under Contract No.DE-AC02-06CH11357. Use of the Lilly Research Laboratories
Collaborative Access Team (LRL-CAT) beamline at Sector 31 of the Advanced Photon
Source was provided by Eli Lilly Company, which operates the facility.
2.7 ACKNOWLEDGEMENTS
We thank Dr. Preyesh Stephen and Dr. Zhen-Kun Sun for language checking. We thank Mr.
Ronald Maheux for the image analysis of the exposed films from the TLC plates. Bo Zhang
thanks the grant provided by CIHR (MOP 97917) and a national scholarship provided by
China Scholarship Council (CSC) for supporting his Ph.D. study. Dr. Xiao-Jian Hu thanks
the National Natural Science Foundation of China (No. 31011120381) for supporting the
international travel expenses for his visiting to Dr. Lin’s laboratory. X-ray diffraction
datasets were collected at LRL-CAT at the Advanced Photon Source, Argonne National
Laboratory.
40
2.8 REFERENCES
1. Miller, W. L. & Auchus, R. J. (2011). The molecular biology, biochemistry, and
physiology of human steroidogenesis and its disorders. Endocr Rev 32, 81-151.
2. Penning, T. M., Jin, Y., Rizner, T. L. & Bauman, D. R. (2008). Pre-receptor
regulation of the androgen receptor. Mol Cell Endocrinol 281, 1-8.
3. Deyashiki, Y., Ogasawara, A., Nakayama, T., Nakanishi, M., Miyabe, Y., Sato, K.
& Hara, A. (1994). Molecular cloning of two human liver 3 alpha-
hydroxysteroid/dihydrodiol dehydrogenase isoenzymes that are identical with
chlordecone reductase and bile-acid binder. Biochem J 299 (Pt 2), 545-52.
4. Khanna, M., Qin, K. N., Wang, R. W. & Cheng, K. C. (1995). Substrate specificity,
gene structure, and tissue-specific distribution of multiple human 3 alpha-
hydroxysteroid dehydrogenases. J Biol Chem 270, 20162-8.
5. Penning, T. M., Burczynski, M. E., Jez, J. M., Hung, C. F., Lin, H. K., Ma, H.,
Moore, M., Palackal, N. & Ratnam, K. (2000). Human 3alpha-hydroxysteroid
dehydrogenase isoforms (AKR1C1-AKR1C4) of the aldo-keto reductase
superfamily: functional plasticity and tissue distribution reveals roles in the
inactivation and formation of male and female sex hormones. Biochem J 351, 67-
77.
6. Dufort, I., Labrie, F. & Luu-The, V. (2001). Human types 1 and 3 3 alpha-
hydroxysteroid dehydrogenases: differential lability and tissue distribution. J Clin
Endocrinol Metab 86, 841-6.
7. Peltoketo, H., Isomaa, V., Maentausta, O. & Vihko, R. (1988). Complete amino
acid sequence of human placental 17 beta-hydroxysteroid dehydrogenase deduced
from cDNA. FEBS Lett 239, 73-7.
8. Luu-The, V., Labrie, C., Zhao, H. F., Couet, J., Lachance, Y., Simard, J., Leblanc,
G., Cote, J., Berube, D., Gagne, R. & et al. (1989). Characterization of cDNAs for
human estradiol 17 beta-dehydrogenase and assignment of the gene to chromosome
17: evidence of two mRNA species with distinct 5'-termini in human placenta. Mol
Endocrinol 3, 1301-9.
41
9. Ghosh, D., Pletnev, V. Z., Zhu, D. W., Wawrzak, Z., Duax, W. L., Pangborn, W.,
Labrie, F. & Lin, S. X. (1995). Structure of human estrogenic 17 beta-
hydroxysteroid dehydrogenase at 2.20 Å resolution. Structure 3, 503-13.
10. Agarwal, A. K., Monder, C., Eckstein, B. & White, P. C. (1989). Cloning and
expression of rat cDNA encoding corticosteroid 11 beta-dehydrogenase. J Biol
Chem 264, 18939-43.
11. Rizner, T. L., Lin, H. K., Peehl, D. M., Steckelbroeck, S., Bauman, D. R. &
Penning, T. M. (2003). Human type 3 3alpha-hydroxysteroid dehydrogenase (aldo-
keto reductase 1C2) and androgen metabolism in prostate cells. Endocrinology 144,
2922-32.
12. Davies, P. & Eaton, C. L. (1991). Regulation of prostate growth. J Endocrinol 131,
5-17.
13. Zhang, Y., Dufort, I., Rheault, P. & Luu-The, V. (2000). Characterization of a
human 20alpha-hydroxysteroid dehydrogenase. J Mol Endocrinol 25, 221-8.
14. Nishizawa, M., Nakajima, T., Yasuda, K., Kanzaki, H., Sasaguri, Y., Watanabe, K.
& Ito, S. (2000). Close kinship of human 20alpha-hydroxysteroid dehydrogenase
gene with three aldo-keto reductase genes. Genes Cells 5, 111-25.
15. Dufort, I., Soucy, P., Labrie, F. & Luu-The, V. (1996). Molecular cloning of human
type 3 3 alpha-hydroxysteroid dehydrogenase that differs from 20 alpha-
hydroxysteroid dehydrogenase by seven amino acids. Biochem Biophys Res
Commun 228, 474-9.
16. Dufort, I., Rheault, P., Huang, X. F., Soucy, P. & Luu-The, V. (1999).
Characteristics of a highly labile human type 5 17beta-hydroxysteroid
dehydrogenase. Endocrinology 140, 568-74.
17. Lin, H. K., Jez, J. M., Schlegel, B. P., Peehl, D. M., Pachter, J. A. & Penning, T. M.
(1997). Expression and characterization of recombinant type 2 3 alpha-
hydroxysteroid dehydrogenase (HSD) from human prostate: demonstration of
bifunctional 3 alpha/17 beta-HSD activity and cellular distribution. Mol Endocrinol
11, 1971-84.
18. Nahoum, V., Gangloff, A., Legrand, P., Zhu, D. W., Cantin, L., Zhorov, B. S., Luu-
The, V., Labrie, F., Breton, R. & Lin, S. X. (2001). Structure of the human 3alpha-
42
hydroxysteroid dehydrogenase type 3 in complex with testosterone and NADP at
1.25-A resolution. J Biol Chem 276, 42091-8.
19. Jin, Y., Stayrook, S. E., Albert, R. H., Palackal, N. T., Penning, T. M. & Lewis, M.
(2001). Crystal structure of human type III 3alpha-hydroxysteroid
dehydrogenase/bile acid binding protein complexed with NADP(+) and
ursodeoxycholate. Biochemistry 40, 10161-8.
20. Couture, J. F., de Jesus-Tran, K. P., Roy, A. M., Cantin, L., Cote, P. L., Legrand, P.,
Luu-The, V., Labrie, F. & Breton, R. (2005). Comparison of crystal structures of
human type 3 3alpha-hydroxysteroid dehydrogenase reveals an "induced-fit"
mechanism and a conserved basic motif involved in the binding of androgen.
Protein Sci 14, 1485-97.
21. Hoog, S. S., Pawlowski, J. E., Alzari, P. M., Penning, T. M. & Lewis, M. (1994).
Three-dimensional structure of rat liver 3 alpha-hydroxysteroid/dihydrodiol
dehydrogenase: a member of the aldo-keto reductase superfamily. Proc Natl Acad
Sci U S A 91, 2517-21.
22. Matsuura, K., Deyashiki, Y., Sato, K., Ishida, N., Miwa, G. & Hara, A. (1997).
Identification of amino acid residues responsible for differences in substrate
specificity and inhibitor sensitivity between two human liver dihydrodiol
dehydrogenase isoenzymes by site-directed mutagenesis. Biochem J 323 (Pt 1), 61-
4.
23. Zhu, D. W., Cantin, L., Nahoum, V., Rehse, P., Luu-The, V., Labrie, F., Breton, R.
& Lin, S. X. (2001). Crystallization and preliminary X-ray crystallographic analysis
of the human type 3 3 alpha-hydroxysteroid dehydrogenase at 1.8 Å resolution.
Acta Crystallogr D Biol Crystallogr 57, 589-91.
24. Battye, T. G., Kontogiannis, L., Johnson, O., Powell, H. R. & Leslie, A. G. (2011).
iMOSFLM: a new graphical interface for diffraction-image processing with
MOSFLM. Acta Crystallogr D Biol Crystallogr 67, 271-81.
25. Winn, M. D., Ballard, C. C., Cowtan, K. D., Dodson, E. J., Emsley, P., Evans, P. R.,
Keegan, R. M., Krissinel, E. B., Leslie, A. G., McCoy, A., McNicholas, S. J.,
Murshudov, G. N., Pannu, N. S., Potterton, E. A., Powell, H. R., Read, R. J., Vagin,
43
A. & Wilson, K. S. (2011). Overview of the CCP4 suite and current developments.
Acta Crystallogr D Biol Crystallogr 67, 235-42.
26. Vagin, A. & Teplyakov, A. Molecular replacement with MOLREP. (2010). Acta
Crystallogr D Biol Crystallogr 66, 22-5.
27. Vagin, A. A., Steiner, R. A., Lebedev, A. A., Potterton, L., McNicholas, S., Long,
F. & Murshudov, G. N. (2004). REFMAC5 dictionary: organization of prior
chemical knowledge and guidelines for its use. Acta Crystallogr D Biol Crystallogr
60, 2184-95.
28. Emsley, P. & Cowtan, K. (2004). Coot: model-building tools for molecular
graphics. Acta Crystallogr D Biol Crystallogr 60, 2126-32.
29. Laskowski, R. A., Macarthur, M. W., Moss, D. S. & Thornton, J. M. (1993).
Procheck - a Program to Check the Stereochemical Quality of Protein Structures.
Journal of Applied Crystallography 26, 283-291.
30. Gangloff, A., Shi, R., Nahoum, V. & Lin, S. X. (2003). Pseudo-symmetry of C19
steroids, alternative binding orientations, and multispecificity in human estrogenic
17beta-hydroxysteroid dehydrogenase. FASEB J 17, 274-6.
31. Couture, J. F., Legrand, P., Cantin, L., Luu-The, V., Labrie, F. & Breton, R. (2003).
Human 20alpha-hydroxysteroid dehydrogenase: crystallographic and site-directed
mutagenesis studies lead to the identification of an alternative binding site for C21-
steroids. J Mol Biol 331, 593-604.
32. Bennett, M. J., Albert, R. H., Jez, J. M., Ma, H., Penning, T. M. & Lewis, M.
(1997). Steroid recognition and regulation of hormone action: crystal structure of
testosterone and NADP+ bound to 3 alpha-hydroxysteroid/dihydrodiol
dehydrogenase. Structure 5, 799-812.
33. Di Costanzo, L., Drury, J. E., Christianson, D. W. & Penning, T. M. (2009).
Structure and catalytic mechanism of human steroid 5beta-reductase (AKR1D1).
Mol Cell Endocrinol 301, 191-8.
34. Hara, A., Matsuura, K., Tamada, Y., Sato, K., Miyabe, Y., Deyashiki, Y. & Ishida,
N. (1996). Relationship of human liver dihydrodiol dehydrogenases to hepatic bile-
acid-binding protein and an oxidoreductase of human colon cells. Biochem J 313
(Pt 2), 373-6.
44
35. Steckelbroeck, S., Jin, Y., Gopishetty, S., Oyesanmi, B. & Penning, T. M. (2004).
Human cytosolic 3alpha-hydroxysteroid dehydrogenases of the aldo-keto reductase
superfamily display significant 3beta-hydroxysteroid dehydrogenase activity:
implications for steroid hormone metabolism and action. J Biol Chem 279, 10784-
95.
36. Jin, Y. & Penning, T. M. (2006). Molecular docking simulations of steroid
substrates into human cytosolic hydroxysteroid dehydrogenases (AKR1C1 and
AKR1C2): insights into positional and stereochemical preferences. Steroids 71,
380-91.
37. Chen, M., Drury, J. E., Christianson, D. W. & Penning, T. M. (2012). Conversion of
human steroid 5beta-reductase (AKR1D1) into 3beta-hydroxysteroid
dehydrogenase by single point mutation E120H: example of perfect enzyme
engineering. J Biol Chem 287, 16609-22.
38. Jin, Y. & Penning, T. M. (2006). Multiple steps determine the overall rate of the
reduction of 5alpha-dihydrotestosterone catalyzed by human type 3 3alpha-
hydroxysteroid dehydrogenase: implications for the elimination of androgens.
Biochemistry 45, 13054-63.
39. Velica, P., Davies, N. J., Rocha, P. P., Schrewe, H., Ride, J. P. & Bunce, C. M.
(2009). Lack of functional and expression homology between human and mouse
aldo-keto reductase 1C enzymes: implications for modelling human cancers. Mol
Cancer 8, 121.
40. Higaki, Y., Usami, N., Shintani, S., Ishikura, S., El-Kabbani, O. & Hara, A. (2003).
Selective and potent inhibitors of human 20alpha-hydroxysteroid dehydrogenase
(AKR1C1) that metabolizes neurosteroids derived from progesterone. Chem Biol
Interact 143-144, 503-13.
41. Takahashi, R. H., Grigliatti, T. A., Reid, R. E. & Riggs, K. W. (2009). The effect of
allelic variation in aldo-keto reductase 1C2 on the in vitro metabolism of
dihydrotestosterone. J Pharmacol Exp Ther 329, 1032-9.
42. Arthur, J. W. & Reichardt, J. K. (2010). Modeling single nucleotide polymorphisms
in the human AKR1C1 and AKR1C2 genes: implications for functional and
genotyping analyses. PLoS One 5, e15604.
45
43. Ma, H. & Penning, T. M. (1999). Conversion of mammalian 3alpha-hydroxysteroid
dehydrogenase to 20alpha-hydroxysteroid dehydrogenase using loop chimeras:
changing specificity from androgens to progestins. Proc Natl Acad Sci U S A 96,
11161-6.
46
Table 2.1 Data collection and refinement statistics
Structure
3α-HSD3
NADP+·progesterone
3α-HSD3 V54L
NADP+·progesterone
A. Data collection
Unit cell dimensions
a, b, c (Å)
β, α=γ (degrees)
52.80, 86.82, 76.49
105.96, 90.00
53.14, 87.10, 76.87
106.31, 90.00
Space group P21 P21
Resolution range (Å) 21.50-2.20 (2.32-2.20) 25.00-2.00 (2.11-2.00)
Total reflections 123,942 (17,392) 159,275 (20,993)
Unique reflections 32,561 (4701) 44,885 (6376)
Completeness (%) 96.4 (95.9) 98.7 (96.6)
Rmerge a
0.037 (0.056) 0.037 (0.053)
I/σ(I) 26.4 (19.3) 19.2 (14.2)
B. Refinement statistics
Reflection used (R-free set) 30,919 (1640) 42,617 (2263)
R-factor b
0.146 0.140
R-free c
0.194 0.183
Root mean square deviations
Bond lengths (Å)
Bond angles (degrees)
0.017
1.902
0.019
1.941
Protein atoms d
NADP+ molecules
d
Steroid molecules d
Sulfate ion d
Water molecules d
5204
2
2
2
369
5206
2
2
2
544
Average B-factors (Å2)
All atoms
Protein atoms e
11.8
10.0/12.8
11.1
8.9/12.4
47
NADP+ e
9.8/11.4 7.9/10.4
Steroid e
Sulfate ion e
Water
37.7/34.4
13.4/24.2
14.7
23.3/27.6
14.9/26.3
17.6
Ramachandran statistics (%) f
Most favored regions
Additionally allowed regions
Generously allowed regions
Disallowed regions
93.1
6.6
0.0
0.3
93.6
6.1
0.0
0.3
a Rmerge = ΣΣi|I(h)-I(h)i|/ΣΣiI(h),where I(h) is the mean intensity after rejections.
b R-factor = Rcryst = Σ(|FO|-|FC|)/Σ|FO|, where |FO| and |FC| are the observed and calculated
structure factor amplitudes for the reflection with Miller indices h = (h, k, l), respectively.
c R-free is calculated for a “test” set of reflections, which was not included in refinement.
d Per asymmetric unit.
e Average B-factors were calculated separately for two monomers within an asymmetric
unit (monomer A/monomer B).
f Ramachandran statistics was calculated with PROCHECK in COOT. Ser221 in both
monomers of human 3α-HSD3 were found in the disallowed regions 18
.
48
Table 2.2 Steady-state kinetic parameters for 5α-DHT and progesterone reduction
catalyzed by the wild type (WT) 3α-HSD3 and the Val54Leu (V54L) mutant in the
presence of NADPH
Enzyme Substrate Km (μM) kcat (min-1
) kcat/Km (min-1
μM-1
)
3α-HSD3 WT 5α-DHT 2.18 ± 0.03 3.67 1.68
3α-HSD3 V54L 5α-DHT 71.03 ± 0.65 6.92 0.10
3α-HSD3 WT Progesterone 0.84 ± 0.01 0.21 0.25
3α-HSD3 V54L Progesterone 2.13 ± 0.13 2.35 1.10
49
Figure 2.1 Structure of the 3α-HSD3·NADP+·progesterone complex
(A) The crystal asymmetric unit contains two monomers. Monomer A is colored in
magenta. Monomer B is colored in cyan. Atoms are colored as follows. Green, carbon
atoms of steroids and cofactors; blue, nitrogen; red, oxygen; orange, phosphorus. (B) The
steroid binding site of monomer A. The 2Fo-Fc electron density map around progesterone
is contoured at 0.9 σ level. Protein carbon is colored in magenta. A water molecule is
located at the catalytic site. (C) The steroid binding site of monomer B. The 2Fo-Fc
electron density map around progesterone is contoured at 0.7 σ level. Protein carbon is
colored in cyan. Hydrogen bonds in (B) and (C) are shown by black dashed lines. (D)
Superposition of the steroid binding sites of monomer A and B. For clarity, carbon atoms of
steroids and cofactors in monomer A and B are colored in magenta and cyan, respectively.
Progesterone possesses two binding conformations in the steroid binding site of the wild
type enzyme.
50
51
52
Figure 2.2 Structure of the 3α-HSD3 V54L·NADP+·progesterone complex
(A) The steroid binding site of monomer A in the 3α-HSD3 V54L·NADP+·progesterone
complex. The 2Fo-Fc electron density map around progesterone is contoured at 1.1 σ level.
Atoms are colored as follows. Green, carbon; blue, nitrogen; red, oxygen; orange,
phosphorus. Protein chain is colored in green. A water molecule is located at the catalytic
site. Hydrogen bonds are shown by black dashed lines. (B) Superposition of the steroid
binding sites of monomer A and B in the 3α-HSD3 V54L·NADP+·progesterone complex.
Carbon and protein chain of monomer B are colored in dark gray. Progesterone possesses
only one binding conformation in the steroid binding site of the mutant enzyme.
53
54
Figure 2.3 Presence of the reduced form of the cofactor NADPH within the purified
protein samples of the wild type 3α-HSD3 and the V54L mutant
Lane 1, 14
C-5α-DHT marker; lane 2, the wild type 3α-HSD3 with 14
C-5α-DHT in the
reaction mixture; lane 3, the V54L mutant with 14
C-5α-DHT in the reaction mixture; lane 4,
14C-progesterone marker; lane 5, the wild type 3α-HSD3 with
14C-progesterone in the
reaction mixture; lane 6, the V54L mutant with 14
C-progesterone in the reaction mixture.
55
Figure 2.4 Superposition of the steroid binding sites of human 3α-HSD3 related
structures
(A) Superposition of the steroid binding sites of two monomer A in the 3α-
HSD3·NADP+·progesterone complex (colored as in Figure 2.1(D)) and the 3α-HSD3
V54L·NADP+·progesterone complex (colored as in Figure 2.2(A)). (B) Superposition of
the steroid binding site of monomer A in the 3α-HSD3 V54L·NADP+·progesterone
complex (colored as in Figure 2.2(A)) and that of the 20α-HSD·NADP+·20α-OHProg
complex (PDB code 1MRQ; carbon and protein chain are colored in orange). (C)
Superposition of the steroid binding site of monomer B in the 3α-
HSD3·NADP+·progesterone complex (colored as in Figure 2.1(D)) and that of the 3α-
HSD3·NADP+·ursodeoxycholate complex (PDB code 1IHI; carbon and protein chain are
colored in pink). (D) Superposition of the steroid binding site of monomer A in the 3α-
HSD3 V54L·NADP+·progesterone complex and that of the 3α-
HSD3·NADP+·ursodeoxycholate complex.
56
57
58
59
CHAPTER 3 STRUCTURE CLUES OF 5ΑLPHA-DHT
ALTERNATIVE BINDING WITHIN HUMAN 3ΑLPHA-HSD3 AND
THE ROLE OF THE ENZYME IN BREAST CANCER
60
3.0 PREFACE
The most potent androgen 5α-DHT has been shown to reduce breast cancer cell growth and
human 3α-HSD3 plays an essential role to inactivate 5α-DHT. However, the important
structural information about the interaction of 3α-HSD3 with its substrate 5α-DHT is still
not available. Also, the role of 3α-HSD3 in breast cancer cells is short of investigations. By
combining the X-ray crystallography and the functional studies in the cellular level, we
carry out the research on these issues.
This chapter includes one paper: Human 3-alpha hydroxysteroid dehydrogenase type 3:
structural clues of 5α-DHT alternative binding and enzyme down-regulation decreasing
breast cancer cell growth. In this paper, I carried out all the experimental studies except for
the work indicated below and wrote the manuscript. I and Dr. Xiao-Jian Hu solved the
crystal structure of the 3α-HSD3·NADP+·A-dione/epi-ADT complex. I solved the crystal
structure of the 3α-HSD3·NADP+·4-dione complex. Mr. Xiang-Qiang Wang and I used the
ELISA kit to determine the 5α-DHT concentration. Dr. Dao-Wei Zhu guided the protein
purification. The q-RTPCR was done by the q-RTPCR platform (Centre Hospitalier
Universitaire (CHU) de Quebec Research Center (CHUL) and Laval University, Québec).
The GC/MS analysis was done by the bioanalytical platform (Centre Hospitalier
Universitaire (CHU) de Quebec Research Center (CHUL) and Laval University, Québec).
Dr. Sheng-Xiang Lin and I designed the study.
61
Human 3-alpha hydroxysteroid dehydrogenase type 3: structural clues of
5α-DHT alternative binding and enzyme down-regulation decreasing
breast cancer cell growth
Bo Zhang 1, 2
, Xiao-Jian Hu 3, Xiao-Qiang Wang
1, Dao-Wei Zhu
1, Peng Shang
2, Fernand
Labrie 1, Sheng-Xiang Lin
1, §
1 Laboratory of Molecular Endocrinology and Oncology, Centre Hospitalier Universitaire
(CHU) de Quebec Research Center (CHUL) and Laval University, Québec City, Québec,
G1V4G2, Canada
2 Key Laboratory for Space Bioscience & Biotechnology, Institute of Special
Environmental Biophysics, School of Life Sciences, Northwestern Polytechnical University,
Xi’an, P. R. China, 710072
3 School of Life Sciences, Fudan University, Shanghai, P.R. China, 200433
§ Corresponding Author: S.-X. Lin, CHUL Research Center, 2705 Boul. Laurier, Québec
City, QC, G1V4G2, Canada; Tel.: +1 418 654 2296
E-mail: [email protected]
Shortened title: Structure clues of 5α-DHT alternative binding within human 3α-HSD3 and
the role of the enzyme in breast cancer
62
3.1 ABSTRACT
Human 3-alpha hydroxysteroid dehydrogenase type 3 (3α-HSD3) plays essential roles in
steroid hormone metabolism, especially in the inactivation of the most potent androgen 5α-
DHT. Besides, 5α-DHT has been shown to reduce breast cancer cell growth. However, the
important structural information about 3α-HSD3 inactivation of 5α-DHT is still not
available and the role of 3α-HSD3 in breast cancer cells is short of investigations. Here, we
reported the crystal structure of human 3α-HSD3·NADP+·A-dione/epi-ADT complex,
which was obtained by co-crystallization with 5α-DHT in the presence of NADP+.
Although 5α-DHT was introduced during the crystallization, the oxidoreduction of 5α-DHT
occurred. A-dione and epi-ADT were identified to be located in the steroid binding sites of
two monomers (monomer A and B) in a crystal asymmetric unit, respectively. An overlay
showed that A-dione and epi-ADT were oriented upside down and flipped to each other,
which provided the structural clues of 5α-DHT alternative binding within the enzyme to
yield different products. Moreover, we reported the crystal structure of the 3α-
HSD3·NADP+·4-dione complex. Using a crystallization condition without the acetate ion,
the crystal was obtained by co-crystallization with testosterone in the presence of NADP+.
The acetate ion introduced from the crystallization condition could distort the steroid
binding conformation and it should be avoided. In addition, using specific siRNA to knock
down 3α-HSD3 expression in MCF7 breast cancer cells, 5α-DHT concentration increased
while MCF7 cell growth was suppressed.
Keywords: 3α-HSD3, AKR1C2, crystal structure, 5α-DHT, alternative binding, cancer cell
growth
Protein data bank accession codes: 4NNE and 4NNF
63
3.2 INTRODUCTION
Breast cancer is a common steroid-related cancer in women 1; 2
. According to the statistics
of the American and Canadian Cancer Society, breast cancer is the second leading cause of
death from cancer in women in North America. 17β-estradiol (E2), the most potent
estrogen, stimulates the proliferation of breast cancer cells, whereas androgen 5α-
dihydrotestosterone (5α-DHT) can reduce breast cancer cell growth 3; 4; 5; 6; 7
. As known, 5α-
DHT is the most potent androgen, and is highly involved in the development of prostate
cancer 8; 9; 10; 11
. In human, 3-alpha hydroxysteroid dehydrogenase type 3 (3α-HSD3) plays a
major role of 5α-DHT reduction to produce the inactive steroid 5α-androstan-3α,17β-diol
(3α-diol) in the presence of NADPH 12; 13; 14
, which makes 3α-HSD3 acting as a pre-
receptor regulator of androgen receptor (AR) in prostate cancer 15; 16; 17; 18
. However, the
role of 3α-HSD3 in breast cancer cells is short of investigations.
There are four isoenzymes (types 1, 2, 3 and 4) included in human 3-alpha hydroxysteroid
dehydrogenase family (3α-HSDs), which belongs to the aldo-keto reductase (AKR)
superfamily and are also named AKR 1C4, 1C3, 1C2 and 1C1, respectively 19; 20
. These
isoenzymes have varying degrees of 3-keto-, 17-keto-, and 20-ketosteroid reductase
activities to inactivate androgens, progestins, and bile acid precursors 18; 21; 22
. They are
highly homologous enzymes and show differential tissue distributions 13; 22; 23
. Human 3α-
HSD1 (AKR1C4) is a liver-specific enzyme acting on the steroid metabolism in liver 22; 23
.
Human 3α-HSD2 (AKR1C3) is highly expressed in prostate and mammary glands, and
shows a major ability to biosynthesize testosterone (Testo) from 4-androsten-3,17-dione (4-
dione) 24; 25
. Human 3α-HSD3 (AKR1C2) is expressed in several tissues including liver,
lung, brain, prostate, testis, mammary gland and adrenal 13; 22
. In vitro, 3α-HSD3 can
oxidize 3α-diol to 5α-DHT in the presence of NAD+. However, it practically acts as a
reductase to inactivate 5α-DHT depending upon the cellular environment 13; 14; 26
. Human
3α-HSD3 is also recognized as the bile acid binding protein and can be inhibited by bile
acids such as ursodeoxycholate 27; 28
. In the pathogenesis of female hirsutism, a reduced
expression of 3α-HSD3 along with an elevated 5α-DHT level is found in tissue of hirsute
women 29
. Human 3α-HSD4 (AKR1C1, also called 20-alpha hydroxysteroid
dehydrogenase (20α-HSD)) is found in mammary gland, ovary, uterus and placenta, and
64
predominantly exerts its 20-ketosteroid reductase activity to inactivate progesterone 22; 30; 31
.
It is noteworthy that 3α-HSD3 and 3α-HSD4 share 97.8% sequence identity, and only
seven residues are different between two enzymes. However, they show distinctive
specificity for steroidal substrates.
The former crystal structures of 3α-HSD3 show that this enzyme possesses an (α/β)8-barrel
motif, and its steroid binding pocket possesses considerable flexibility, which is formed by
five loops including loop A (residues 117-143), loop B (residues 217-238), loop C (residues
299-323), and two short loops (residues 23-32 and 51-57) 32; 33; 34
. Although these structures
provide the detailed information, the crucial structure of 3α-HSD3 in complex with 5α-
DHT is still not available
In this study, we reported the high-resolution crystal structure of the 3α-HSD3·NADP+·A-
dione/epi-ADT complex, which was obtained by co-crystallization with 5α-DHT.
Surprisingly, the oxidoreduction of 5α-DHT occurred during the crystallization process and
produced a mixture of steroids. A-dione and epi-ADT were identified to be located in the
enzyme cavities. Moreover, we reported the crystal structure of the 3α-HSD3·NADP+·4-
dione complex. Using a crystallization condition without the acetate ion, the steroid binding
conformation was more reasonable and less distorted. In addition, using specific siRNA to
knockdown 3α-HSD3 expression in breast cancer cells, the impacts of 3α-HSD3 expression
on the concentration of 5α-DHT and cell proliferation were further investigated.
3.3 MATERIALS AND METHODS
3.3.1 Materials
MCF7 cells and MTT cell proliferation assay kit were purchased from the American Type
Culture Collection (ATCC). Fetal bovine serum (FBS, Qualified, US origin) and
Lipofectamine 2000 transfection reagent were purchased from Life Technologies
Corporation. Dulbecco’s Modified Eagle’s Medium (DMEM) low-glucose medium was
ordered from Sigma-Aldrich. siRNA was ordered from Shanghai GenePharma. 5α-DHT
ELISA kit was ordered from Alpha Diagnostic International. 5α-DHT and Testo were
ordered from Steraloids. Diethyl ether, acetone, toluene and dichloromethane were
65
purchased from Fisher Scientific. Thin layer chromatography (TLC) plate was purchased
from EMD Millipore. 14
C-labelled 5α-DHT (53.5 mCi/mmol) was purchased from
PerkinElmer Life Sciences. 14
C-labelled Testo (55 mCi/mmol) was purchased from
American Radiolabeled Chemicals. NADPH, NADP+ and other chemicals were purchased
from Sigma-Aldrich.
3.3.2 Protein purification and crystallization
Human 3α-HSD3 was purified basically following a previously reported procedure 35
.
Briefly, the recombinant enzyme with a glutathione S-transferase (GST) tag was initially
purified with a glutathione agarose column and then the second step of purification by the
Q-sepharose column can fulfill the task. The enzyme was concentrated to about 30 mg/ml
in a 10 mM KH2PO4-K2HPO4 buffer (pH 7.0) containing 0.5 mM DTT, 0.06% β-OG, 1
mM EDTA, 1 mM NADP+, 40 μM 5α-DHT or 40 μM Testo. Crystals were obtained in the
sitting drops by using the vapor diffusion method at room temperature. Before
crystallization, 5α-DHT or Testo were added into the 0.5 ml well solution to reach the final
1 mM concentration, respectively, and the crystallization condition included 100 mM
sodium cacodylate (pH 6.0), 200 mM ammonium sulfate, 24-26% (w/v) polyethylene
glycol (PEG) 3350. Crystals appeared after three days and then reached to their full size
within two weeks. During the crystallization period, 5α-DHT can be oxidized to A-dione
and then be reduced to epi-ADT by the enzyme. The well solution containing 15% glycerol
was selected as the cryoprotective solution.
3.3.3 Data collection and structure determination
The X-ray diffraction data were collected at beamline 31-ID-D (λ= 0.979 Å) of the
Advanced Photon Source (APS) at Argonne National Laboratory. Data sets were indexed
and integrated by iMosflm 36
. Both space groups of the 3α-HSD3·NADP+·A-dione/epi-
ADT complex and the 3α-HSD3·NADP+·4-dione complex were P21. There are two
monomers (A and B) contained in an asymmetric unit for each crystal structure. In the 3α-
HSD3·NADP+·A-dione/epi-ADT complex, A-dione was found in monomer A and epi-
ADT was found in monomer B (see “RESULTS”). Using the reported 3α-HSD3 structure
(PDB code 1J96) 32
, the two crystal structures were solved by molecular replacement with
66
the program Molrep in CCP4 37; 38
. The program Refmac in CCP4 and COOT were used for
refinement and model building, respectively 39; 40
. After the amino acid residues of the
enzyme and water molecules were refined, NADP+ and steroids were fitted into the 2FO-FC
omit electron density and refined. Finally, the quality of the models was verified with
PROCHECK 41
.
3.3.4 The oxidoreduction assay of steroids and the GC/MS analysis
The reaction of 5α-DHT oxidoreduction was performed at 37.0 ± 0.3°C in a volume of 1 ml
25 mM Tris-HCl buffer (pH 7.4) containing 10% Glycerol, 0.1 mM 5α-DHT (with 0.1 μM
14C-labelled 5α-DHT), 1 mM NADP
+ and 0.01 mg/ml of BSA. The reaction was initiated
by adding the enzyme to the reaction mixture, and the final concentration of the enzyme
was 0.2 mg/ml. After overnight incubation, the reaction was terminated by adding 3 ml
diethyl ether. Duplicates of reactions were performed. Following a standard TLC protocol
42, steroids were separated. TLC plate was exposed and quantified by a Storm imaging
system. Similarly, the reaction of Testo oxidation was performed using the same
experimental condition as the reaction of 5α-DHT oxidoreduction except that 5α-DHT and
14C-labelled 5α-DHT were replaced by Testo and
14C-labelled Testo. In addition, the
reaction mixture of 5α-DHT oxidoreduction (without 14
C-labelled 5α-DHT) was analyzed
by gas chromatography and mass spectrometer (GC/MS). The GC/MS analysis was carried
out by the bioanalytical platform (Centre Hospitalier Universitaire (CHU) de Québec
Research Center (CHUL), Université Laval, Québec, Canada).
3.3.5 Cell culture
MCF7 cells were cultured in DMEM low-glucose medium in the presence of 10% FBS and
the medium was phenol red-free. Cells were maintained in a humidified incubator at 37°C
and supplied with 5% CO2. When indicated, FBS was treated with 2% (w/v) dextran-coated
charcoal overnight at 4°C to deprive the original steroids in FBS.
3.3.6 siRNA synthesis and transfection
Human 3α-HSD3 siRNA (sense: AAGCUCUAGAGGCCGUCAAAUTT; antisense:
AUUUGACGGCCUCUAGAGCUUTT) was designed according to the previous research
67
43 and the specificity of siRNA was checked by BLAST in human genome
44. Duplex 3α-
HSD3 siRNA and negative control (NC) siRNA were synthesized and purified with HPLC
by Shanghai GenePharma. siRNA was transfected by using lipofectamine 2000 and
following the manufacturer’s protocol.
3.3.7 Quantitative real-time RT-PCR
MCF7 cells were plated into a six-well plate at 4 × 105 cells per well with 2 ml medium and
cultured one bay before siRNA transfection. MCF7 cells were transfected with 100 nM 3α-
HSD3 specific siRNA or negative control siRNA for 24 hours and then cells were treated
with Trizol reagent. The treated samples were sent to the q-RTPCR platform (Centre
Hospitalier Universitaire (CHU) de Québec Research Center (CHUL), Université Laval,
Québec, Canada) for the mRNA quantification of 3α-HSD3 and 3α-HSD4. The primer
sequences of 3α-HSD3 (5’-CCTAAAAGTAAAGCTCTAGAGGCCGT-3’; 5’-CAACTCT-
GGTCGATGGGAATTGCT-3’) and 3α-HSD4 (5’-AAAGTAAAGCTTTAGAGGCC-
ACC-3’; 5’-AAATGAATAAGGTAGAGGTCAACATAA-3’) were designed based on the
previous studies 26; 45
.
3.3.8 Determination of 5α-DHT levels by Elisa assay
MCF7 cells were seeded into 24-well plate at 50,000 cells per well with 0.5 ml medium
treated with dextran-coated charcoal. After cultured for 24 hours, cells were transfected
with 100 nM 3α-HSD3 specific siRNA or negative control siRNA and grown for another
48 hours. Then, the cell culture medium was replaced with fresh charcoal treated medium
containing 0.7 nM 5α-DHT. Supernatants of the cell culture medium were collected after
48 hours. Following the protocol of its supplier, 5α-DHT levels in supernatants were
determined by using a commercial 5α-DHT ELISA kit.
3.3.9 Cell proliferation assay
Cell proliferation was determined by MTT (3-(4, 5-dimethylthiazol-2-yl)-2, 5-
diphenyltetrazolium bromide) assay. MCF7 cells were seeded into 24-well plate as the way
used in Elisa assay and cultured for 24 hours. Next, cells were transfected with 100 nM 3α-
HSD3 specific siRNA or negative control siRNA. After another 24 hours cell culture, the
68
culture medium was replaced with fresh charcoal treated medium containing different
concentrations of 5α-DHT (0.1 nM or 1.0 nM). Cell growth study was performed for 96
hours and the medium was replaced every 48 hours. MTT assay was carried out as
described previously 7. Absorbance was read at 570 nm with a reference at 650 nm.
3.4 RESULTS
3.4.1 Crystal growth of human 3α -HSD3 in complex with A-dione/epi-ADT and 4-dione
5α-DHT is the main steroid transformed by human 3α-HSD3. However, its complex
structure with the enzyme is still not available. At the beginning, crystal growth of human
3α-HSD3 in complex with 5α-DHT has been performed using the reported crystallization
condition, which includes 100 mM sodium citrate (pH 5.6), 260 mM ammonium acetate, 1
mM 5α-DHT, 26-27% (w/v) polyethylene glycol (PEG) 4000 32
. After obtaining the
crystal, the solved crystal structure showed that acetate and citrate molecules were deeply
bound in the steroid binding site, while 5α-DHT could not be observed. The whole
structure resembles the reported human 3α-HSD3·NADP+·citrate/acetate complex
34. To
solve this problem, the crystallization condition was adjusted to 100 mM sodium
cacodylate (pH 6.0), 200 mM ammonium sulfate, 1 mM 5α-DHT and 24-26% (w/v)
polyethylene glycol (PEG) 3350. By doing so, the crystal was obtained and the electron
density of the steroid was shown in the steroid binding site. Surprisingly, the solved
structure shows that the bound steroids can be fitted with A-dione and epi-ADT, but not
with 5α-DHT. The oxidoreduction of 5α-DHT happened during the crystallization and a
mixture of steroids including A-dione and epi-ADT were generated (Figure 3.1), which
phenomenon was also observed in human steroid 5β-reductase co-crystallization with 5α-
DHT 46
. In addition, in the previously reported 3α-HSD3·NADP+·Testo/acetate complex
32,
the acetate molecule with high concentration (260 mM) from the crystallization condition
saturates the active site of the enzyme and can distort the actual steroid binding
conformation. Therefore, human 3α-HSD3 has been co-crystallized with Testo by using an
adjusted crystallization condition without the acetate molecule.
69
3.4.2 Overall structures of human 3α-HSD3 in complex with A-dione/epi-ADT and 4-
dione
The crystal structures of the 3α-HSD3·NADP+·A-dione/epi-ADT complex and the 3α-
HSD3·NADP+·4-dione complex both possess the monoclinic space group of P21, and there
are two monomers (A and B) included in an asymmetric unit (Figure 3.2(A)). The 3α-
HSD3·NADP+·A-dione/epi-ADT complex was refined at 1.20 Å with a crystallographic R-
factor of 15.5% and an Rfree-factor of 17.4%. The 3α-HSD3·NADP+·4-dione complex was
refined at 1.75 Å with an R-factor of 16.4% and an Rfree-factor of 20.5%. The protein
backbones of two complexes are quite similar to each other and the root mean square
deviations (RMSD) of the backbone Cα atoms in both monomer A is 0.42 Å. However,
loop A (residues 117-143) of two complexes undergoes a considerable conformational
variation and the RMSD value for 27 Cα atoms of loop A in both monomer A is 1.32 Å. It
is noteworthy that monomer A owns a lower thermal B-factor than that of monomer B in
two complexes. The cofactor is tightly bound in the enzyme with an extended conformation
and its binding mode is almost unchanged in different complexes 32; 33; 34
. Numbers of
hydrogen bonds, salt bridges and Van der Waals interactions contribute to the stabilization
of NADP+ in the enzyme as described previously
32; 33. The Ramachandran plot shows that
above 93% residues of two complexes are located in the most favored regions. Data
collection and refinement statistics are summarized in Table 3.1.
3.4.3 Human 3α-HSD3 in complex with A-dione/epi-ADT
The human 3α-HSD3·NADP+·A-dione/epi-ADT complex was obtained by co-
crystallization in the presence of 5α-DHT. The difference Fourier map defines that two
different steroids exist in the cavity of monomer A and B, respectively. In monomer A, A-
dione well depicts the majority of electron density map with the lower average B-factors. In
monomer B, epi-ADT agrees with the electron density map with the lower average B-
factors. However, partially weak electron density can also be found to accommodate epi-
ADT in monomer A, and correspondingly, a similar phenomenon can be observed in
monomer B. Nevertheless, A-dione and epi-ADT represent the major steroid binding mode
in monomer A and B, respectively, and were determined in the structure. To be surprised,
although 5α-DHT was introduced during the crystallization, the observed electron density
70
defined that A-dione or epi-ADT bound into the cavity. Thus, reactions that simulating the
crystallization condition were performed by following the instructions in “METHODS”.
The results show that 5α-DHT is oxidized to A-dione in the presence of 1 mM NADP+, and
then 5α-DHT and A-dione are reduced to 3α-diol/3β-diol and ADT/epi-ADT, respectively
(Figure 3.1). With the overnight incubation, A-dione and epi-ADT hold the percentage of
26% and 17% among the mixture of steroids. Moreover, the GC/MS analysis further
indicates that the outputs ratio of 3α-diol/3β-diol and ADT/epi-ADT are about 2.2:1 and
2.1:1, respectively.
In monomer A, the O17 atom of A-dione is oriented toward the nicotinamide ring of
NADP+ (Figure 3.2(B)). The α-face of A-dione interacts with the side chains of Val54 and
Val128. Its β-face mainly interacts with the indole ring of Trp227, and the steroid C18 and
C19 methyl groups are pointing toward Trp227. It is worth mentioning that a water
molecule is located at the catalytic core and forms hydrogen bonds with the side chains of
Tyr55, His117 and the O17 atom of A-dione. In monomer B, the O3 atom of epi-ADT is
pointing toward the nicotinamide ring (Figure 3.2(C)). The α-face of epi-ADT is stacking
with the indole ring of Trp227, and the steroid C18 and C19 methyl groups are pointing
toward Val54 and Tyr55. Particularly, the O3 atom of epi-ADT forms a hydrogen bond
with His222 Nε atom. When monomer A and B are superimposed, the O3 and O17 atoms of
both steroids are oriented upside down to each other, and the planes of both steroids are
flipped about 145° around the long axis of C3-C17 (Figure 3.2(D)). After superposition, the
RMSD value is 0.43 Å for their backbone Cα atoms. In both monomers, loop A and a short
loop (residues 23-33) possess considerable fluctuation and the RMSD values for their Cα
atoms are 1.06 Å and 1.05 Å, respectively. The residues of Val54, Tyr55, His 117, His222
and Leu308, which belong to the steroid binding pocket, are relatively static, while the side
chains of Val128, Ile129 and Leu306 display apparent movement to consort with steroids.
In particular, the side chain of Leu306 contains two alternative conformations in both
monomers, which may correspond to the two different orientations of steroids.
3.4.4 Human 3α-HSD3 in complex with 4-dione
The human 3α-HSD3·NADP+·4-dione complex was obtained by co-crystallization with
Testo in the presence of NADP+. During the crystallization process, the oxidation of Testo
71
occured and 4-dione was generated (Figure 3.3). The difference Fourier map clearly shows
that 4-dione is located in the steroid binding site of each monomer (Figure 3.4(A)). When
monomer A and B are superimposed, the orientation and conformation of 4-dione are quite
similar to each other and only a small shift of the steroid plane toward the indole ring of
Trp227 can be observed (Figure 3.4(B)). The backbones of monomer A and B overlap each
other quite well, and the RMSD value for the backbone Cα atom is 0.36 Å. Loop A still
displays its flexibility and the RMSD value for its 27 Cα atom is 0.96 Å. The side chains of
Val54, Val128, Ile129 and Leu308 in the steroid binding pocket also exhibit subtle
adjustments in two monomers. The C3 atom and the A-ring of 4-dione is pointing toward
the nicotinamide ring. The α-face of 4-dione interacts with the side chain of Trp227, and
the C18 and C19 methyl groups of 4-dione are pointing toward the side chain of His117.
The O3 atom of 4-dione forms a hydrogen bond with His222 Nε atom.
Compared with the orientation of Testo in the reported 3α-HSD3·NADP+·Testo/acetate
complex 32
, it can be clearly seen that the plane of 4-dione in the 3α-HSD3·NADP+·4-dione
complex generates an about 45° rotation around its C3-C17 long axis (Figure 3.4(B)).
Meanwhile, the steroid goes deeper into the cavity of the enzyme, and the distance between
the C3 atoms of steroids and the C4 atom of the nicotinamide ring is changed to 4.3 Å from
the former 6.2 Å. The acetate molecule in the Testo/acetate complex, which is originated
from the crystallization condition, is situated between the steroid and the cofactor, and
occupies the catalytic site of the enzyme. Obviously, the repulsion between the O3 atom of
Testo and the ketone group of acetate remarkably twists the steroid orientation. However,
the acetate molecule is replaced by a water molecule in the 4-dione complex, and the latter
forms hydrogen bonds with the side chains of Tyr55 and His117. Moreover, the side chains
of Val54, Ile129, Trp227, Leu306, Leu308 and the nicotinamide ring have slight
adjustments to accommodate the more suitable orientation of the steroid.
3.4.5 3α-HSD3 expression and siRNA specific knockdown in MCF7 cells
The mRNA transcription of human 3α-HSD3 and 3α-HSD4 in MCF7 cells was evaluated
by quantitative RT-PCR. The results show that the mRNA level of 3α-HSD3 is about 2.5
times that of 3α-HSD4 in MCF7 cells (Figure 3.5(A)). Due to the high similarity of 3α-
HSD3 and 3α-HSD4 on the nucleotide sequences, the selective knockdown of the 3α-HSD3
72
expression, without interferencing with 3α-HSD4, was performed by a specific siRNA.
Compared with control siRNA treated cells, the quantitative RT-PCR results show that 3α-
HSD3 specific siRNA significantly suppresses 3α-HSD3 expression, while the expression
of 3α-HSD4 is affected negligibly (Figure 3.5(B)).
3.4.6 Suppression of 3α-HSD3 expression increases 5α-DHT concentration in MCF7
cells
To investigate the impact of 3α-HSD3 expression on 5α-DHT concentration in MCF7 cells,
ELISA assays were carried out using supernatants from the cell culture medium (Figure
3.6(A)). After siRNA treatment, MCF7 cells were cultured for 48 hours with the charcoal
treated medium containing 0.7 nM (203 pg/ml) 5α-DHT. Compared with the control siRNA
treated groups, the 5α-DHT concentration from the 3α-HSD3 specific siRNA treated group
shows significantly higher 5α-DHT concentration (about 154 pg/ml), which is about 2.3
times the value of the control group (about 68 pg/ml).
3.4.7 Suppression of 3α-HSD3 expression decreases MCF7 cell proliferation in the
presence of 5α-DHT
To assess the potential role of 3α-HSD3 on MCF7 cell proliferation, siRNA specific
knockdown of 3α-HSD3 expression in MCF7 cells was performed. After siRNA treatment,
MCF7 cells were cultured for 96 hours with the charcoal treated medium containing 0.1 nM
or 1.0 nM 5α-DHT. Compared with MCF7 cells transfected with control siRNA, MCF7
cells transfected with 3α-HSD3 specific siRNA exhibits significantly decreased growth
rate, with about 20% or 25% reduction of the cell growth under the cultured conditions
containing 1.0 nM or 0.1 nM 5α-DHT, respectively (Figure 3.6(B)).
3.5 DISCUSSION
In order to recognize the molecular characteristics of 5α-DHT binding to human 3α-HSD3,
a high resolution crystal was obtained by co-crystallization in the presence of 5α-DHT and
NADP+. However, during the crystallization process, 5α-DHT initiated a series of
oxidoreduction and generated a mixture of steroids. Therefore, A-dione and epi-ADT were
identified, which located in two monomers (A and B) of the enzyme in a crystal
73
asymmetric unit, respectively. In monomer A, the O17 atom of A-dione is pointing inside
into the catalytic site of the enzyme, which means 5α-DHT has been oxidized on its C17
hydroxyl group to output A-dione and then the generated A-dione resides in the cavity of
the enzyme. In monomer B, the O3 atom of epi-ADT is oriented toward the catalytic site of
the enzyme, which implies that A-dione has been reduced on its C3 carbonyl group to
produce ADT and epi-ADT, while only epi-ADT is retained in the cavity of the enzyme.
Although the assay of 5α-DHT oxidoreduction mimicking the crystallization process shows
that 5α-DHT has also been reduced to 3α-diol and 3β-diol, resembling to ADT, these two
steroids have been released from the cavity after the reactions. Nevertheless, the different
orientations of A-dione and epi-ADT provide the structural clues of 5α-DHT alternative
binding in the cavity of the enzyme to generate different steroids. In addition, both loop A
of monomer A and B possess different neighboring environments from the nearby
symmetric molecules and display an apparent flexibility. In addition, in the 3α-
HSD3·NADP+·4-dione complex, Testo was introduced before crystallization, while the
observed electron density in the cavity agreed with 4-dione. That means the C17 hydroxyl
group of Testo firstly enters into the catalytic site of 3α-HSD3, and Testo is oxidized to 4-
dione in the presence of the cofactor. Then, 4-dione is released from the catalytic site and
reenters with its C3 carbonyl group pointing inside. Interestingly, this process is reversed in
the former 3α-HSD3·NADP+·Testo/acetate complex
32. Therefore, the evidence further
supports the alternative binding modes of steroids in 3α-HSD3.
The alternative binding modes of steroids in enzymes have also been found in other
hydroxysteroid dehydrogenase such as human 17β-hydroxysteroid dehydrogenase type 1
(17β-HSD1), 3α-HSD2 (also named 17β-HSD5 or AKR1C3). In human 17β-HSD1, 5α-
DHT can be oxidized to A-dione and simultaneously be reduced to 3β-diol, which implies
the existence of the alternative binding orientations of 5α-DHT in the enzyme 42
.
Meanwhile, the structural study further verify that androgens such as Testo, A-dione and 4-
dione can bind in reverse orientation within the enzyme compared with the orientations of
estrogens such as 17β-estradiol 42; 47
. In human 3α-HSD2, the crystal structure shows that
two reverse orientations of Testo can be observed in the cavity of the enzyme 48
. Moreover,
for human steroid 5β-reductase (also named AKR1D1), the enzyme E120H mutant was co-
crystallized with 5α-DHT 46
. During the crystallization process, the oxidoreduction of 5α-
74
DHT occurred and produced a mixture of steroids. 3β-diol and epi-ADT were found to
occupy the cavity of monomer A and B in the crystal asymmetric unit, which indicated that
the alternative binding modes of steroids in the enzyme corresponds with the
multispecificity of the enzyme. Taken together, the alternative binding modes of steroids in
the enzyme originates from the pseudo self-symmetry property of steroids and the
flexibility of the steroid binding pocket.
Recently, the reported human 3α-HSD3·NADP+·progesterone complex shows that although
the D-ring of the steroid is pointing toward the cavity of the enzyme, progesterone
possesses two different orientations in the cavity. When superimposed with the 3α-
HSD3·NADP+·A-dione/epi-ADT complex, in both monomer A, the orientations of A-dione
and progesterone resemble with each other, and only the D-rings of two steroids show a
little detachment (Figure 3.7(A)). The C18 and C19 methyl groups of two steroids are
pointing toward Trp227. The side chains of Val54, His222, Leu306 and Leu308 are
flipping about 180°, which reflects the subtle flexibility of the steroid binding site. Besides,
in both monomer B, although the A, B, C and D rings of epi-ADT and progesterone are
located reversely to each other, the orientations of two steroids planes are roughly identical
to each other, and both α-face of steroids interact with the side chain of Trp227 (Figure
3.7(B)). In addition, in the reported 3α-HSD3·NADP+·ursodeoxycholate complex, an
overlay shows that the overall orientation of ursodeoxycholate is similar to that of epi-ADT
in the cavity, and there is only a little swing between two ligands around the vertical axis of
the steroid plane (Figure 3.7(C)). Therefore, two major orientations of steroids can be
found in the cavity of 3α-HSD3, which further implies the steroid binding site of 3α-HSD3
possessing considerable flexibility.
In the 3α-HSD3·NADP+·4-dione complex, the overall conformation of the enzyme is quite
identical to monomer A of the 3α-HSD3·NADP+·progesterone complex, and the RMSD
value is only 0.14 Å between the backbone Cα atoms of both monomer A. Although an
overlay shows that two steroids are oriented back to back as well as their C18 and C19
methyl groups are pointing toward the opposite directions, the orientations of two steroids
resemble with each other (Figure 3.7(D)). This indicates that the steroid binding pocket of
3α-HSD3 has sufficient space and flexibility to allow the planes of steroids flipping inside.
75
Previously, compared with benign tissue, an increased 5α-DHT concentration as well as a
decreased expression of 3α-HSD3 in prostate tumor was observed by Stolz and coworkers
16; 26. They speculated that the loss of 3α-HSD3 in prostate cancer cells increased 5α-DHT
dependent cell growth. As known, through binding to AR, excessive 5α-DHT leads to the
stimulation of prostate cancer proliferation. 3α-HSD3 eliminates 5α-DHT in prostate and
this can prevent AR activation from excessive androgens. In addition, they reported that, in
the presence of progesterone, specific knocking down of 3α-HSD4 alone or with 3α-HSD3
together in T47D cells led to decreased cell growth 43
. The former studies indicate that 5α-
DHT still plays an important role of antiproliferation in breast cancer cells, which is
mediated by AR 5; 6; 49; 50
. Human 3α-HSD3 is characterized by its major ability to
inactivate 5α-DHT, which prompts us to explore its role in breast cancer cells. In this study,
the 3α-HSD3 expression was knocked down by specific siRNA in MCF7 cells, and a
relative elevation of 5α-DHT level was observed by using ELISA assay. Meanwhile, in the
presence of 5α-DHT, suppression of 3α-HSD3 expression by specific siRNA resulted in a
decrease of MCF7 cell growth, which suggested that the suppressed expression of 3α-
HSD3 strengthened the antiproliferative effect of 5α-DHT in MCF7 cells. In addition to the
outstanding ability of estradiol (E2) production, human 17β-hydroxysteroid dehydrogenase
type 1 (17β-HSD1) also displays an ability to inactivate 5α-DHT 42
. Suppression of 17β-
HSD1 expression was shown to increase 5α-DHT level in T47D cells, which showed an
antiproliferative effect 7. However, compared with 5α-DHT inactivation ability of 17β-
HSD1 (Km = 32.0 μM, kcat = 2.40 min-1
and kcat/Km = 0.08 min-1
μM-1
) 42
, 3α-HSD3
possesses a significantly higher activity to reduce 5α-DHT (Km = 1.1 μM, kcat = 1.5 min-1
and kcat/Km = 1.3 min-1
μM-1
) 32
, which implies that 3α-HSD3 may play a more important
role than 17β-HSD1 to inactivate 5α-DHT.
3.6 FUNDING SOURCES
This work was supported by the Canadian Institutes of Health Research (CIHR), with a
grant to Dr. Sheng-Xiang Lin and collaborators (MOP 97917). Use of the Advanced Photon
Source, an Office of Science User Facility operated for the U.S. Department of Energy
(DOE) Office of Science by Argonne National Laboratory, was supported by the U.S. DOE
under Contract No.DE-AC02-06CH11357. Use of the Lilly Research Laboratories
76
Collaborative Access Team (LRL-CAT) beamline at Sector 31 of the Advanced Photon
Source was provided by Eli Lilly Company, which operates the facility. The Canadian
Macromolecular Crystallography Facility (CMCF) is supported by CFI, NSERC, and CIHR.
3.7 ACKNOWLEDGEMENTS
We thank Dr. Donald Poirier for offering us several steroids and the helpful discussions.
We thank Ms. Nathalie Paquet, Mr. Patrick Bélanger for the services of the q-RTPCR
analysis and the GC/MS analysis, who are from the q-RTPCR platform, the bioanalytical
platform (Centre Hospitalier Universitaire (CHU) de Quebec Research Center (CHUL) and
Laval University, Québec), respectively. We thank PROTEO (The Quebec Network for
Research on Protein Function, Structure, and Engineering) and Dr. Albert Berghuis’
laboratory at McGill University for providing the X-ray crystallography facilities for our
initial X-ray datasets collection. We thank Dr. Preyesh Stephen for the revision of the
manuscript. Bo Zhang thanks a national scholarship provided by China Scholarship
Council (CSC) and the CIHR grant (MOP 97917) to support his graduate study. X-ray
diffraction datasets were collected at LRL-CAT at the Advanced Photon Source, Argonne
National Laboratory, and at the CMCF, Canadian Light Source.
77
3.8 REFERENCES
1. Henderson, B. E. & Feigelson, H. S. (2000). Hormonal carcinogenesis.
Carcinogenesis 21, 427-33.
2. Dunn, B. K. & Ford, L. G. (2007). Hormonal interventions to prevent hormonal
cancers: breast and prostate cancers. Eur J Cancer Prev 16, 232-42.
3. Poulin, R., Baker, D. & Labrie, F. (1988). Androgens inhibit basal and estrogen-
induced cell proliferation in the ZR-75-1 human breast cancer cell line. Breast
Cancer Res Treat 12, 213-25.
4. Labrie, F., Luu-The, V., Labrie, C., Belanger, A., Simard, J., Lin, S. X. & Pelletier,
G. (2003). Endocrine and intracrine sources of androgens in women: inhibition of
breast cancer and other roles of androgens and their precursor
dehydroepiandrosterone. Endocr Rev 24, 152-82.
5. Macedo, L. F., Guo, Z., Tilghman, S. L., Sabnis, G. J., Qiu, Y. & Brodie, A. (2006).
Role of androgens on MCF-7 breast cancer cell growth and on the inhibitory effect
of letrozole. Cancer Res 66, 7775-82.
6. Greeve, M. A., Allan, R. K., Harvey, J. M. & Bentel, J. M. (2004). Inhibition of
MCF-7 breast cancer cell proliferation by 5alpha-dihydrotestosterone; a role for
p21(Cip1/Waf1). J Mol Endocrinol 32, 793-810.
7. Aka, J. A., Mazumdar, M., Chen, C. Q., Poirier, D. & Lin, S. X. (2010). 17beta-
hydroxysteroid dehydrogenase type 1 stimulates breast cancer by
dihydrotestosterone inactivation in addition to estradiol production. Mol Endocrinol
24, 832-45.
8. Siiteri, P. K. & Wilson, J. D. (1970). Dihydrotestosterone in prostatic hypertrophy.
I. The formation and content of dihydrotestosterone in the hypertrophic prostate of
man. J Clin Invest 49, 1737-45.
9. Huggins, C. & Hodges, C. V. (1941). Studies on prostatic cancer - I The effect of
castration, of estrogen and of androgen injection on serum phosphatases in
metastatic carcinoma of the prostate. Cancer Res 1, 293-7.
10. Davies, P. & Eaton, C. L. (1991). Regulation of prostate growth. J Endocrinol 131,
5-17.
78
11. Ross, R. K., Pike, M. C., Coetzee, G. A., Reichardt, J. K., Yu, M. C., Feigelson, H.,
Stanczyk, F. Z., Kolonel, L. N. & Henderson, B. E. (1998). Androgen metabolism
and prostate cancer: establishing a model of genetic susceptibility. Cancer Res 58,
4497-504.
12. Dufort, I., Soucy, P., Labrie, F. & Luu-The, V. (1996). Molecular cloning of human
type 3 3 alpha-hydroxysteroid dehydrogenase that differs from 20 alpha-
hydroxysteroid dehydrogenase by seven amino acids. Biochem Biophys Res
Commun 228, 474-9.
13. Dufort, I., Labrie, F. & Luu-The, V. (2001). Human types 1 and 3 3 alpha-
hydroxysteroid dehydrogenases: differential lability and tissue distribution. J Clin
Endocrinol Metab 86, 841-6.
14. Rizner, T. L., Lin, H. K., Peehl, D. M., Steckelbroeck, S., Bauman, D. R. &
Penning, T. M. (2003). Human type 3 3alpha-hydroxysteroid dehydrogenase (aldo-
keto reductase 1C2) and androgen metabolism in prostate cells. Endocrinology 144,
2922-32.
15. Rizner, T. L., Lin, H. K. & Penning, T. M. (2003). Role of human type 3 3alpha-
hydroxysteroid dehydrogenase (AKR1C2) in androgen metabolism of prostate
cancer cells. Chem Biol Interact 143-144, 401-9.
16. Ji, Q., Chang, L., Stanczyk, F. Z., Ookhtens, M., Sherrod, A. & Stolz, A. (2007).
Impaired dihydrotestosterone catabolism in human prostate cancer: critical role of
AKR1C2 as a pre-receptor regulator of androgen receptor signaling. Cancer Res 67,
1361-9.
17. Penning, T. M., Bauman, D. R., Jin, Y. & Rizner, T. L. (2007). Identification of the
molecular switch that regulates access of 5alpha-DHT to the androgen receptor. Mol
Cell Endocrinol 265-266, 77-82.
18. Penning, T. M., Jin, Y., Rizner, T. L. & Bauman, D. R. (2008). Pre-receptor
regulation of the androgen receptor. Mol Cell Endocrinol 281, 1-8.
19. Miller, W. L. & Auchus, R. J. (2011). The molecular biology, biochemistry, and
physiology of human steroidogenesis and its disorders. Endocr Rev 32, 81-151.
20. Jez, J. M., Flynn, T. G. & Penning, T. M. (1997). A new nomenclature for the aldo-
keto reductase superfamily. Biochem Pharmacol 54, 639-47.
79
21. Deyashiki, Y., Ogasawara, A., Nakayama, T., Nakanishi, M., Miyabe, Y., Sato, K.
& Hara, A. (1994). Molecular cloning of two human liver 3 alpha-
hydroxysteroid/dihydrodiol dehydrogenase isoenzymes that are identical with
chlordecone reductase and bile-acid binder. Biochem J 299 (Pt 2), 545-52.
22. Penning, T. M., Burczynski, M. E., Jez, J. M., Hung, C. F., Lin, H. K., Ma, H.,
Moore, M., Palackal, N. & Ratnam, K. (2000). Human 3alpha-hydroxysteroid
dehydrogenase isoforms (AKR1C1-AKR1C4) of the aldo-keto reductase
superfamily: functional plasticity and tissue distribution reveals roles in the
inactivation and formation of male and female sex hormones. Biochem J 351, 67-
77.
23. Khanna, M., Qin, K. N., Wang, R. W. & Cheng, K. C. (1995). Substrate specificity,
gene structure, and tissue-specific distribution of multiple human 3 alpha-
hydroxysteroid dehydrogenases. J Biol Chem 270, 20162-8.
24. El-Alfy, M., Luu-The, V., Huang, X. F., Berger, L., Labrie, F. & Pelletier, G.
(1999). Localization of type 5 17beta-hydroxysteroid dehydrogenase, 3beta-
hydroxysteroid dehydrogenase, and androgen receptor in the human prostate by in
situ hybridization and immunocytochemistry. Endocrinology 140, 1481-91.
25. Luu-The, V., Dufort, I., Pelletier, G. & Labrie, F. (2001). Type 5 17beta-
hydroxysteroid dehydrogenase: its role in the formation of androgens in women.
Mol Cell Endocrinol 171, 77-82.
26. Ji, Q., Chang, L., VanDenBerg, D., Stanczyk, F. Z. & Stolz, A. (2003). Selective
reduction of AKR1C2 in prostate cancer and its role in DHT metabolism. Prostate
54, 275-89.
27. Stolz, A., Hammond, L., Lou, H., Takikawa, H., Ronk, M. & Shively, J. E. (1993).
cDNA cloning and expression of the human hepatic bile acid-binding protein. A
member of the monomeric reductase gene family. J Biol Chem 268, 10448-57.
28. Hara, A., Matsuura, K., Tamada, Y., Sato, K., Miyabe, Y., Deyashiki, Y. & Ishida,
N. (1996). Relationship of human liver dihydrodiol dehydrogenases to hepatic bile-
acid-binding protein and an oxidoreductase of human colon cells. Biochem J 313
(Pt 2), 373-6.
80
29. Steiner, A. Z., Chang, L., Ji, Q., Ookhtens, M., Stolz, A., Paulson, R. J. & Stanczyk,
F. Z. (2008). 3alpha-Hydroxysteroid dehydrogenase type III deficiency: a novel
mechanism for hirsutism. J Clin Endocrinol Metab 93, 1298-303.
30. Zhang, Y., Dufort, I., Rheault, P. & Luu-The, V. (2000). Characterization of a
human 20alpha-hydroxysteroid dehydrogenase. J Mol Endocrinol 25, 221-8.
31. Nishizawa, M., Nakajima, T., Yasuda, K., Kanzaki, H., Sasaguri, Y., Watanabe, K.
& Ito, S. (2000). Close kinship of human 20alpha-hydroxysteroid dehydrogenase
gene with three aldo-keto reductase genes. Genes Cells 5, 111-25.
32. Nahoum, V., Gangloff, A., Legrand, P., Zhu, D. W., Cantin, L., Zhorov, B. S., Luu-
The, V., Labrie, F., Breton, R. & Lin, S. X. (2001). Structure of the human 3alpha-
hydroxysteroid dehydrogenase type 3 in complex with testosterone and NADP at
1.25-A resolution. J Biol Chem 276, 42091-8.
33. Jin, Y., Stayrook, S. E., Albert, R. H., Palackal, N. T., Penning, T. M. & Lewis, M.
(2001). Crystal structure of human type III 3alpha-hydroxysteroid
dehydrogenase/bile acid binding protein complexed with NADP(+) and
ursodeoxycholate. Biochemistry 40, 10161-8.
34. Couture, J. F., de Jesus-Tran, K. P., Roy, A. M., Cantin, L., Cote, P. L., Legrand, P.,
Luu-The, V., Labrie, F. & Breton, R. (2005). Comparison of crystal structures of
human type 3 3alpha-hydroxysteroid dehydrogenase reveals an "induced-fit"
mechanism and a conserved basic motif involved in the binding of androgen.
Protein Sci 14, 1485-97.
35. Zhu, D. W., Cantin, L., Nahoum, V., Rehse, P., Luu-The, V., Labrie, F., Breton, R.
& Lin, S. X. (2001). Crystallization and preliminary X-ray crystallographic analysis
of the human type 3 3 alpha-hydroxysteroid dehydrogenase at 1.8 A resolution.
Acta Crystallogr D Biol Crystallogr 57, 589-91.
36. Battye, T. G., Kontogiannis, L., Johnson, O., Powell, H. R. & Leslie, A. G. (2011).
iMOSFLM: a new graphical interface for diffraction-image processing with
MOSFLM. Acta Crystallogr D Biol Crystallogr 67, 271-81.
37. Vagin, A. & Teplyakov, A. (2010). Molecular replacement with MOLREP. Acta
Crystallogr D Biol Crystallogr 66, 22-5.
81
38. Winn, M. D., Ballard, C. C., Cowtan, K. D., Dodson, E. J., Emsley, P., Evans, P. R.,
Keegan, R. M., Krissinel, E. B., Leslie, A. G., McCoy, A., McNicholas, S. J.,
Murshudov, G. N., Pannu, N. S., Potterton, E. A., Powell, H. R., Read, R. J., Vagin,
A. & Wilson, K. S. (2011). Overview of the CCP4 suite and current developments.
Acta Crystallogr D Biol Crystallogr 67, 235-42.
39. Vagin, A. A., Steiner, R. A., Lebedev, A. A., Potterton, L., McNicholas, S., Long,
F. & Murshudov, G. N. (2004). REFMAC5 dictionary: organization of prior
chemical knowledge and guidelines for its use. Acta Crystallogr D Biol Crystallogr
60, 2184-95.
40. Emsley, P. & Cowtan, K. (2004). Coot: model-building tools for molecular
graphics. Acta Crystallogr D Biol Crystallogr 60, 2126-32.
41. Laskowski, R. A., Macarthur, M. W., Moss, D. S. & Thornton, J. M. (1993).
Procheck - a Program to Check the Stereochemical Quality of Protein Structures. J
Appl Crystallogr 26, 283-291.
42. Gangloff, A., Shi, R., Nahoum, V. & Lin, S. X. (2003). Pseudo-symmetry of C19
steroids, alternative binding orientations, and multispecificity in human estrogenic
17beta-hydroxysteroid dehydrogenase. FASEB J 17, 274-6.
43. Ji, Q., Aoyama, C., Nien, Y. D., Liu, P. I., Chen, P. K., Chang, L., Stanczyk, F. Z.
& Stolz, A. (2004). Selective loss of AKR1C1 and AKR1C2 in breast cancer and
their potential effect on progesterone signaling. Cancer Res 64, 7610-7.
44. Altschul, S. F., Madden, T. L., Schaffer, A. A., Zhang, J., Zhang, Z., Miller, W. &
Lipman, D. J. (1997). Gapped BLAST and PSI-BLAST: a new generation of
protein database search programs. Nucleic Acids Res 25, 3389-402.
45. Blouin, K., Richard, C., Brochu, G., Hould, F. S., Lebel, S., Marceau, S., Biron, S.,
Luu-The, V. & Tchernof, A. (2006). Androgen inactivation and steroid-converting
enzyme expression in abdominal adipose tissue in men. J Endocrinol 191, 637-49.
46. Chen, M., Drury, J. E., Christianson, D. W. & Penning, T. M. (2012). Conversion of
human steroid 5beta-reductase (AKR1D1) into 3beta-hydroxysteroid
dehydrogenase by single point mutation E120H: example of perfect enzyme
engineering. J Biol Chem 287, 16609-22.
82
47. Shi, R. & Lin, S. X. (2004). Cofactor hydrogen bonding onto the protein main chain
is conserved in the short chain dehydrogenase/reductase family and contributes to
nicotinamide orientation. J Biol Chem 279, 16778-85.
48. Qiu, W., Zhou, M., Labrie, F. & Lin, S. X. (2004). Crystal structures of the
multispecific 17beta-hydroxysteroid dehydrogenase type 5: critical androgen
regulation in human peripheral tissues. Mol Endocrinol 18, 1798-807.
49. Lanzino, M., Sisci, D., Morelli, C., Garofalo, C., Catalano, S., Casaburi, I.,
Capparelli, C., Giordano, C., Giordano, F., Maggiolini, M. & Ando, S. (2010).
Inhibition of cyclin D1 expression by androgen receptor in breast cancer cells--
identification of a novel androgen response element. Nucleic Acids Res 38, 5351-65.
50. Wang, Y., He, X., Yu, Q. & Eng, C. (2013). Androgen receptor-induced tumor
suppressor, KLLN, inhibits breast cancer growth and transcriptionally activates
p53/p73-mediated apoptosis in breast carcinomas. Hum Mol Genet 22, 2263-72.
83
Table 3.1 Data collection and refinement statistics
Structure 3α-HSD3
NADP+·A-dione/epi-ADT
3α-HSD3
NADP+·4-dione
A. Data collection
Unit cell dimensions
a, b, c (Å)
β, α=γ (degrees)
54.64, 86.95, 76.72
107.10, 90.00
52.90, 86.65, 76.99
106.25, 90.00
Space group P21 P21
Resolution range (Å) 17.64-1.20 (1.26-1.20) 25.00-1.75 (1.84-1.75)
Total reflections 759,961 (102,820) 238,631 (32,176)
Unique reflections 212,070 (30,491) 66,677 (9455)
Completeness (%) 99.4 (98.1) 99.3 (97.0)
Rmerge a
0.063 (0.334) 0.089 (0.260)
I/σ(I) 9.8 (3.3) 9.4 (4.2)
B. Refinement statistics
Reflection used (R-free set) 201,387 (10,646) 63,276 (3382)
R-factor b
0.155 0.164
R-free c
0.174 0.205
Root mean square deviations
Bond lengths (Å)
Bond angles (degrees)
0.028
2.590
0.023
2.404
Protein atoms d
NADP+ molecules
d
Steroid molecules d
Sulfate ion d
Water molecules d
5293
2
2
2
832
5165
2
2
2
335
Average B-factors (Å2)
All atoms
Protein atoms e
NADP+ e
12.8
10.8/11.4
9.6/10.5
13.7
12.2/14.2
10.9/13.1
Steroid e
24.6/26.0 28.4/33.4
84
Sulfate ion e
Water
8.3/8.8
23.4
19.3/25.6
19.2
Ramachandran statistics (%) f
Most favored regions
Additionally allowed regions
Generously allowed regions
Disallowed regions
93.6
6.1
0.0
0.3
94.9
4.7
0.0
0.3
a Rmerge = ΣΣi|I(h)-I(h)i|/ΣΣiI(h), where I(h) is the mean intensity after rejections.
b R-factor = Rcryst = Σ(|FO|-|FC|)/Σ|FO|, where |FO| and |FC| are the observed and calculated
structure factor amplitudes for the reflection with Miller indices h = (h, k, l), respectively.
c R-free is calculated for a “test” set of reflections, which was not included in refinement.
d Per asymmetric unit.
e Average B-factors were calculated separately for two monomers within an asymmetric
unit (monomer A/monomer B).
f Ramachandran statistics was calculated with PROCHECK in COOT. Ser221 in both
monomers of human 3α-HSD3 were found in the disallowed regions.
85
Figure 3.1 The oxidoreduction of 5α-DHT catalyzed by human 3α-HSD3 in the
presence of cofactors
(A) Reactions catalyzed by human 3α-HSD3 in the presence of cofactors. (B) An assay
mimicking the crystallization condition in the presence of NADP+ and
14C-labelled 5α-
DHT. Lane 1, the reaction without 3α-HSD3; lane 2, the reaction with 3α-HSD3.
Compared with the migration of different steroids (Anne Gangloff et al., FASEB J.,
2003,17(2):274-6), the results showed that the oxidoreduction of 5α-DHT occurred during
the crystallization and produced a mixture of products that including A-dione, ADT, epi-
ADT, 3α-diol, 3β-diol. These products were further validated by the GC/MS analysis.
86
Figure 3.2 Structure of the 3α-HSD3·NADP+·A-dione/epi-ADT complex
(A) The crystal asymmetric unit contains two monomers. Monomer A colored in magenta
is the 3α-HSD3·NADP+·A-dione complex. Monomer B colored in cyan is the 3α-
HSD3·NADP+·epi-ADT complex. Atoms are colored as follows. Green, carbon atoms of
steroids and cofactors; blue, nitrogen; red, oxygen; orange, phosphorus. (B) The steroid
binding site of monomer A. The 2Fo-Fc electron density map around A-dione is contoured
at 0.7 σ level. Protein carbon is colored in magenta. A water molecule is located at the
catalytic site. (C) The steroid binding site of monomer B. The 2Fo-Fc electron density map
around epi-ADT is contoured at 0.7 σ level. Protein carbon is colored in cyan. Hydrogen
bonds in (B) and (C) are shown by black dashed lines. (D) Superposition of the steroid
binding sites of monomer A and B. For clarity, carbon atoms of steroids and cofactors in
monomer A and B are colored in magenta and cyan, respectively. The planes of A-dione
and epi-ADT are oriented upside down and flipped.
87
88
89
Figure 3.3 The oxidation of testosterone catalyzed by human 3α-HSD3 in the
presence of NADP+
(A) Reactions catalyzed by human 3α-HSD3 in the presence of cofactors. (B) An assay
mimicking the crystallization condition in the presence of NADP+
and 14
C-labelled Testo.
Lane 1, the reaction without 3α-HSD3; lane 2, the reaction with 3α-HSD3. The result
showed that the oxidation of Testo occurred during the crystallization and 4-dione was
generated.
90
Figure 3.4 Structure of the 3α-HSD3·NADP+·4-dione complex
(A) The steroid binding site of monomer A in the 3α-HSD3·NADP+·4-dione complex. The
2Fo-Fc electron density map around 4-dione is contoured at 0.8 σ level. Atoms are colored
as follows. Green, carbon; blue, nitrogen; red, oxygen; orange, phosphorus. Protein chain is
colored in green. A water molecule is located at the catalytic site. Hydrogen bonds are
shown by black dashed lines. (B) Superposition of the steroid binding sites of monomer A
and B in the 3α-HSD3·NADP+·4-dione complex, and that of monomer A in the 3α-
HSD3·NADP+·Testo/acetate complex (PDB code 1J96; carbon and protein chain are
colored in orange; an acetate molecule is located at the catalytic site and distorts the steroid
binding conformation). Carbon and protein chain of monomer B in the 3α-
HSD3·NADP+·4-dione complex are colored in dark gray.
91
92
Figure 3.5 Human 3α-HSD3 expression and knockdown by siRNA in MCF7 cells
(A) The relative mRNA levels of human 3α-HSD3 and 3α-HSD4 in MCF7 cells were
evaluated by quantitative RT-PCR. (B) Compared with the control siRNA treated cells, the
quantitative RT-PCR results showed that 3α-HSD3 specific siRNA substantially
suppressed 3α-HSD3 expression but not 3α-HSD4. Experiments were repeated three times.
93
Figure 3.6 Suppression of 3α-HSD3 in MCF7 cells enhanced 5α-DHT-mediated
inhibition of cell growth
(A) After siRNA transfection, MCF7 cells were cultured for 48 hours with the charcoal-
treated medium containing 0.7 nM (203 pg/ml) 5α-DHT. Steroid concentrations were
determined by ELISA assay using supernatants from the cell culture medium. Compared
with the control siRNA treated groups, the 5α-DHT concentration from the 3α-HSD3
specific siRNA treated group showed significantly increased 5α-DHT concentration.
Experiments were repeated three times in triplicate. (B) After siRNA transfection, MCF7
cells were cultured for 96 hours with the charcoal-treated medium containing 0.1 nM or 1.0
nM 5α-DHT. Cell growth was evaluated by MTT assay. Experiments were repeated three
times in triplicate.
94
Figure 3.7 Superposition of the steroid binding sites of the related 3α-HSD3
structures
(A) Superposition of the steroid binding sites of two monomer A in the 3α-
HSD3·NADP+·A-dione/epi-ADT complex (carbon and protein chain are colored in
magenta) and the 3α-HSD3·NADP+·progesterone complex (carbon and protein chain are
colored in dark gray). The other atoms are colored as follows. Blue, nitrogen; red, oxygen;
orange, phosphorus. (B) Superposition of the steroid binding sites of two monomer B in the
3α-HSD3·NADP+·A-dione/epi-ADT complex (carbon and protein chain are colored in
cyan) and the 3α-HSD3·NADP+·progesterone complex (carbon and protein chain are
colored in orange). (C) Superposition of the steroid binding sites of two monomer B in the
3α-HSD3·NADP+·A-dione/epi-ADT complex and the 3α-HSD3·NADP
+·ursodeoxycholate
complex (carbon and protein chain are colored in pink). (D) Superposition of the steroid
binding sites of two monomer A in the 3α-HSD3·NADP+·4-dione complex (carbon and
protein chain are colored in green) and the 3α-HSD3·NADP+·progesterone complex.
95
96
97
CHAPTER 4 PURIFICATION AND PRELIMINARY
CRYSTALLOGENESIS OF HUMAN ESTROGEN RECEPTOR
ALPHA
98
4.0 PREFACE
Although there are more than twenty years of the structural studies on estrogen receptor
alpha (ERα), due to the difficulties in protein expression, purification and crystallization,
the full-length ERα structure remains an unfulfilled task. Recently, more and more studies
showed that the DNA binding domain (DBD) and the ligand binding domain (LBD) of
nuclear receptors (NRs), which including ERα DBD and LBD, exerted their functions as a
whole. The mechanism of bi-directional regulation between ERα DBD and LBD should be
investigated further. Therefore, we determined to establish an expression and purification
protocol of the ERα fragment containing its DBD-LBD domain, and to crystallize ERα
DBD-LBD in complex with estrogen response elements (EREs).
In addition, several methods have been developed previously to purify ERα LBD, such as
carboxymethylations or mutations of reactive cysteine residues of ERα LBD. During the
purification, the target protein was found mainly existing in the precipitate. Therefore, we
developed a simple and efficient purification method for ERα LBD, which used a
combination of detergents to purify ERα LBD from the precipitate.
This chapter includes two papers: (1) Expression, purification and preliminary
crystallogenesis of human estrogen receptor alpha DBD-LBD. In this paper, I carried out
the experimental studies and wrote the manuscript. Dr. Sheng-Xiang Lin and I designed the
study. (2) A simple and efficient purification method for human estrogen receptor alpha
LBD. In this paper, I carried out the experimental studies and wrote the manuscript. Mr.
Jean-François Thériault, as a summer student, prepared some SDS-PAGE gels. Dr. Sheng-
Xiang Lin, Dr. Dao-Wei Zhu and I designed the study.
99
4.1 EXPRESSION, PURIFICATION AND PRELIMINARY
CRYSTALLOGENESIS OF HUMAN ESTROGEN RECEPTOR ALPHA
DBD-LBD
Expression, purification and preliminary crystallogenesis of human
estrogen receptor alpha DBD-LBD
Bo Zhang 1, 2
, Sheng-Xiang Lin 1, §
1 Laboratory of Molecular Endocrinology and Oncology, Centre Hospitalier Universitaire
(CHU) de Quebec Research Center (CHUL) and Laval University, Québec City, Québec,
G1V4G2, Canada
2 Key Laboratory for Space Bioscience & Biotechnology, Institute of Special
Environmental Biophysics, School of Life Sciences, Northwestern Polytechnical University,
Xi’an, P. R. China, 710072
§ Corresponding Author: S.-X. Lin, CHUL Research Center, 2705 Boul. Laurier, Québec
City, QC, G1V4G2, Canada; Tel.: +1 418 654 2296
E-mail: [email protected]
Shortened title: purification and preliminary crystallogenesis of human ERα DBD-LBD
100
4.1.1 Abstract
Through binding to 17β-estradiol, estrogen receptor alpha (ERα) forms a homodimer and
translocates from the cytoplasm into nucleus to initialize the transcription of specific genes.
ERα plays important physiological functions in human such as controlling sexual
development and reproductive functions. Due to difficulties in protein expression,
purification and crystallization, the full-length ERα structure remains an unfulfilled task. In
this study, we established an expression and purification protocol of the ERα fragment
containing the DNA binding domain and the ligand binding domain (DBD-LBD) of ERα.
Initially, ERα DBD-LBD with the C530A single point mutation was expressed in E.coli
Rosetta2 (DE3) cells. The expression temperature for the target protein was optimized at
25 °C for 12 hours, and 0.2 mM IPTG was used to induce the target protein for expression
in the supernatant with an acceptable quantity. During the purification, the target protein
was prone to aggregation. High salt concentration was found significantly preventing the
protein aggregation and increasing the solubility of ERα DBD-LBD. Through two steps of
purification by the nickel column and the gel filtration column, ERα DBD-LDB was
concentrated to 6.0 mg/ml with the purity above 95%. Preliminary crystallogenesis of ERα
DBD-LBD in complex with estrogen response elements (EREs) was performed. This study
provided basic knowledge to facilitate the acquisition of the fine crystals for ERα DBD-
LBD in complex with EREs.
Keywords: estrogen receptor alpha (ERα), the DNA binding domain (DBD), the ligand
binding domain (LBD), detergent, purification, preliminary crystallogenesis.
101
4.1.2 Introduction
Estrogen receptor alpha (ERα) is a well defined member of Nuclear Receptor superfamily
(NRs). Through binding to 17β-estradiol (E2), ERα controls sexual development and
reproductive functions, and also affects bone, cardiovascular, immune and central nervous
systems 1. Similar to all the members of NRs, ERα contains five structural regions: the N-
terminal region (A/B region: 1-180 amino acids (aa)), the DNA binding domain (DBD or C
region: 181-263aa), the hinge region (D region: 264-302aa), the ligand binding domain
(LBD or E region: 303-552aa), and the C-terminal region (F region: 553-595aa).
The structural studies on NRs LBDs and DBDs have been carried out for more than twenty
years. The solution and crystal structures of ERα DBD without or with estrogen response
elements (EREs) were firstly reported by Schwabe et al 2; 3; 4
. Several years later, the crystal
structures of ERα LBD bound to agonists, antagonists and coactivator were released 5; 6; 7
.
Together with other reported NRs DBDs and LBDs, these structures provided remarkable
insights into the structural and functional basis of NRs and significantly improved the
knowledge of rational drug design against these targets 8; 9; 10; 11; 12; 13; 14; 15
. However, the
purification processes of NRs DBDs and LBDs are full of challenges. NRs DBDs are prone
to aggregation and their solubility is relatively low in solutions 16
. NRs LBDs are unstable
in the absence of their ligands. In particularly, ERα LBD is notorious for aggregation due to
three reactive cysteine residues (Cys381, Cys417 and Cys530). Several methods have been
developed to purify ERα LBD such as carboxymethylation or mutation of cysteine residues
5; 6; 17, denaturation and renaturation
7, or application of reducing agents or fusion protein
18;
19.
Due to the difficulties in protein expression, purification and crystallization, the full-length
NRs structure remains unfulfilled 20
. In 2008, Rastinejad’s group reported the first full-
length structures of intact NRs (PPARγ-RXRα heterodimer) bound to their DNA target 21
.
They found that PPARγ LBD directly impacted the binding of PPARγ DBD to its DNA
elements, which challenged the long-held notion that the NRs DBDs and LBDs maintained
their autonomous and self-reliant functions. Recently, Figueira et al. also reported that
thyroid receptor (TR) DBD-LBD had a higher binding affinity to its DNA elements than
the isolated DBD 22
. Furthermore, the hormone response elements, possessing specific
102
DNA sequences, can regulate ligands binding and receptor activation 15; 23; 24
. Thus, the
mechanism of bidirectional regulation between NRs DBDs and LBDs should be exploited
in depth. It is obvious that only the PPARγ-RXRα heterodimer structure is not adequate to
provide a model that how NRs homodimers are assembled to exert their functions properly.
More structural studies are required to fully understand the functional relationship between
NRs DBDs and LBDs. It has been well established that the N-terminal region of ERα is
intrinsically disordered and this part does not have a stable conformation. Therefore,
expression, purification and preliminary crystallogenesis of human ERα DBD-LBD are the
objectives of this study.
4.1.3 Methods
4.1.3.1 Plasmids construction
The human full-length ERα plasmid was purchased from Genecopoeia (Shanghai, China).
Two nucleotide sequences encoding ERα 179-554aa (amino acids) and 179-595aa were
amplified by PCR and were inserted into the pGEM-T vector, respectively, which included
ERα DBD-LBD. The unique forward primer contained the BamHI site: 5’-
CGCGGATCCGCCAAGGAGACTCGCTAC-3’ and each of the two reverse primers
contained the XhoI site: 5’-CCGCTCGAGTTAGCTAGTGGGCGCATGT-3’, 5’-
CCGCTCGAGTCAGACCGTGGCAGGG-3’. After validation by sequencing, the
recombinant pGEM-T vectors were digested with BamHI and XhoI, and two nucleotide
segments encoding ERα DBD-LBD were cloned into the corresponding sites of the pET-
28a(+) vectors.
4.1.3.2 Site-directed mutagenesis of ERα C530A
The recombinant pET-28a(+) vectors encoding human ERα 179-554aa and 179-595aa were
used as the templates for conducting the site-directed mutagenesis of C530A. The
mutations were carried out by using QuikChange Lightning Kit (Agilent Technologies)
with 5’-CTGTACAGCATGAAGGCCAAGAACGTGGTGCC-3’ as forward primer and
verified by sequencing.
4.1.3.3 Protein expression and purification
103
The pET-28a(+) constructs encoding ERα 179-554aa and 179-595aa with the C530A single
point mutations were expressed in E.coli Rosetta2 (DE3) cells. LB medium was
supplemented with 50 μg/ml kanamycin and 35 μg/ml chloramphenicol. The cells were
cultivated at 37 °C for 3 hours until OD600 reached 0.7, and protein expression was induced
with 0.2 mM isopropyl-β-D-thiogalactopyranoside (IPTG) for an additional 12 hours at
25 °C in the presence of 20 μM estradiol. The cells were harvested by centrifugation and
the pellets were stored at -80 °C. The frozen cells were thawed in buffer A (50 mM Tris-
HCl (pH 7.4), 10 mM imidazole, 500 mM NaCl, 10% glycerol, 20 mM β-mercaptoethanol,
1 mM phenylmethylsulfonyl fluoride (PMSF), 20 μM estradiol, 0.1% β-OG (β-Octyl
glucoside)) with the addition of 1 mg/ml lysozyme and 1 μg/ml each of protease inhibitors
(leupeptin, chymostatin, antipain, aprotinin, pepstatin A and benzamidin). After incubation
on ice for 20 minutes, the cells were lysed by sonication. The supernatant was obtained via
centrifugation at 181,000 g for 50 minutes and loaded onto a 3 ml Ni-NTA agarose column
pre-equilibrated with buffer A, followed by incubation at 4 °C for 3 hours. Afterwards, the
nickel column was washed with buffer A containing an imidazole gradient from 30 mM to
200 mM. Peak fractions were pooled and concentrated using an ultra centrifugal filter with
a 30 kDa molecular-weight cutoff (Millipore). Further separation was achieved by running
the gel filtration on a Sephacryl S-200 column previously equilibrated in buffer A without
imidazole. The eluted fractions were concentrated and the buffer was exchanged to 25 mM
Tris-HCl (pH 7.4), 250 mM NaCl, 80 mM MgCl2, 5 μM zinc chloride, 10% glycerol, 2.5
mM DTT, 20 μM estradiol and 0.1% β-OG, by three rounds of dilution and concentration.
The purity of the concentrated ERα 179-554aa and 179-595aa was estimated by SDS-
PAGE. The protein concentration was determined by the Bradford method.
4.1.3.4 Solubility test
The E.coli cells containing the ERα DBD-LBD recombinant plasmids were grown at 37 °C
in 200 ml LB media for 2.5 hours until OD600 reached 0.6. Next, the expression of the
target protein was induced with 0.2 mM, 0.5 mM or 1.0 mM IPTG at 37 °C for 4 hours or
at 18 °C overnight in the presence of 20 μM estradiol. The cell pellets were harvested and
resuspended in 10 ml buffer A, followed by sonication and centrifugation. The supernatant
was discarded. The precipitate was resuspended again in 10 ml buffer A without 0.1% β-
104
OG and each solubility test used 0.5 ml resuspended sample. 0.4% (w/v) each of Triton X-
100, C12E8 (Octaethylene glycol monododecyl ether), β-DDM (dodecyl-β-D-maltoside), β-
OG, Emulgen913 or 0.5 M NDSB-201 (Non detergent sulfobetaines) was added to the 0.5
ml sample, respectively. Each sample was slowly agitated overnight at 4 °C and the results
were verified by SDS-PAGE.
4.1.3.5 Western blot analysis
Western blot was performed using primary rabbit anti-ERα polyclonal antibody (ab70170)
(Abcam) with a 1:10,000 dilution. Horseradish peroxidase-conjugated secondary goat anti-
rabbit antibody (Santa Cruz Biotechnology) was utilized by a 1:7,500 dilution. Protein
signal was detected with ECL reagents (PerkinElmer) and exposed to chemiluminescence
film (GE Healthcare).
4.1.3.6 Preliminary test of crystallization
To obtain the crystal of ERα DBD-LBD in complex with EREs, PAGE purified single-
stranded EREs were purchased from IDT Company and resuspended in 50 mM Tris-HCl
buffer (pH 7.4), 100 mM NaCl. Next, the complementary EREs strands were mixed
together at a 1:1 molar ratio, heated to 95 °C and then annealed to 5 °C over 4 hours. The
purified ERα 179-554aa and 179-595aa mixed with the double-stranded EREs at a 2:1.2
molar ratio. The crystallization was performed using the vapor diffusion method in a
hanging drop at room temperature and 4 °C. The Nextal screen (Qiagen), the Natrix screen
(Hampton Research) and several homemade screen conditions were used for the
preliminary crystallogenesis.
4.1.4 Results and discussion
4.1.4.1 Construction, expression and solubility test of ERα DBD-LBD
Following the procedures in Methods, two DNA fragments encoding human ERα DBD-
LBD (179-554aa and 179-595aa) were cloned into pET-28a(+) vector, respectively (Figure
4.1.1). The recombinant vectors with the mutations of C530A were validated by sequencing.
105
After transforming the E.coli BL21 (DE3) competent cells with the recombinant vectors,
the expression of ERα DBD-LBD was induced by 0.5 mM IPTG at 37 °C for 4 hours. Due
to a lack of the target protein expression, the E. coli Rosetta2 (DE3) competent cells were
tested as an alternative. The E. coli Rosetta2 strains contained seven tRNAs rare codons
and the expression of the target protein was appeared (Figure 4.1.2). Next, the cells were
cultivated at 37 °C until OD600 reached 0.6, and then the expression of target protein was
induced with different concentrations of IPTG at 0.2 mM, 0.5 mM, 1.0 mM and cultured
for 4 hours at 37 °C. However, after sonication and centrifugation, the target protein was
present mostly in the precipitate, not in the supernatant. Therefore, several commonly used
detergents were used for the protein solubility test. The equivalent precipitate was
resuspended in buffer A, each containing 0.4% of Triton X-100, C12E8, β-DDM, β-OG,
Emulgen913 or 0.5M NDSB-201, respectively, and slowly agitated at 4 °C overnight. After
centrifugation, the target protein was still present in the sediment. So, in this case, these
detergents had little efficacy for improving the solubility of ERα DBD-LBD (data not
shown here). Furthermore, the cells were grown at 37 °C for 3 hours until OD600 reached
0.7 and the expression of ERα 179-595aa was induced with 0.2 mM IPTG at 18 °C for 20
hours. The lower temperature facilitated the expression of the target protein in the
supernatant, but the quantity was relatively low (Figure 4.1.3(A)). Meanwhile, the
solubility tests for the precipitate treated with different detergents were also carried out and
the results showed that detergents had little effect. Finally, 0.2mM IPTG as well as a cell
culture for 12 hours at 25 °C were used to induce the expression of ERα DBD-LBD to an
acceptable quantity in the supernatant (Figure 4.1.3(B)).
4.1.4.2 Purification of ERα DBD-LBD
The frozen pellets from 2 liters of the E.coli cells expressing ERα DBD-LBD were thawed
in buffer B (50 mM Tris-HCl (pH 8.0), 10 mM imidazole, 200 mM NaCl, 10% glycerol, 20
mM β-mercaptoethanol, 1 mM PMSF and 20 μM estradiol) with the addition of lysozyme
and protease inhibitors. After sonication and centrifugation, the supernatant was loaded
onto the nickel column and incubated at 4 °C to assist binding for 3 hours. The target
protein was eluted with buffer B containing 200 mM imidazole and 0.1% β-OG. However,
immediately following the elution, the target protein began to aggregate. To address this
106
problem, the solubility test was performed. 0.4% (w/v) each of Triton X-100, C12E8, β-
DDM, β-OG, Emulgen913 or 0.5 M NDSB-201 was employed to improve the solubility of
the target protein. Only NDSB-201 was found to be mildly efficacious. Interestingly, high
salt concentrations (above 400 mM NaCl) were found to significantly increase the
solubility of ERα DBD-LBD. Thus, buffer A containing 500 mM NaCl was ultimately used
to purify the target protein instead of buffer B. Following the procedures as mentioned
above, the supernatant sample was loaded onto the nickel column and the column was
washed with buffer A containing a gradient of imidazole concentration from 30 mM to 80
mM. Then, the target protein was eluted with buffer A containing 200 mM imidazole. After
the nickel column purification, further step of purification was achieved by using a
Sephacryl S-200 gel filtration column (Figure 4.1.4). ERα DBD-LBD was concentrated to
0.5ml of 6.0 mg/ml in a buffer containing 25 mM Tris-HCl (pH 7.4), 250 mM NaCl, 80
mM MgCl2, 5 μM zinc chloride, 10% glycerol, 2.5 mM DTT, 20 μM estradiol and 0.1% β-
OG. The purity of the protein was estimated by SDS-PAGE and above 95%. This protocol
was applied to the purification of both ERα DBD-LBD fragments (179-554aa and 179-
595aa). In addition, a Western blot was performed to further verify the target band
representing ERα DBD-LBD.
4.1.4.3 Preliminary crystallogenesis of ERα DBD-LBD
Before crystallization, single stands of EREs were annealed to form a palindrome DNA
segment and then mixed with ERα DBD-LBD (179-554aa) at a 1.2:2 molar ratio. 96
conditions of the Nextal screen were initially used to crystallize ERα DBD-LBD (179-
554aa) in complex with EREs at room temperature and at 4 °C, yet no protein crystal was
obtained. Later, the Natrix screen was used to grow the crystal and was still not successful.
Then, by adjusting some crystallization conditions from the related studies 3; 21; 25; 26; 27; 28
,
several uniquely designed crystallization conditions were tested to grow the crystal. A
number of tiny needle crystals appeared at 4 °C after two weeks in one optimized
crystallization condition, which contained 7.5% (w/v) PEG3350 in 0.1 M MES buffer (pH
7.0) with 0.1 M MgCl2 and 0.2 M NaCl (Figure 4.1.5). The needle crystals were too tiny to
be scooped out from the hanging drop for SDS-PAGE verification, but they were unlikely
to be salt crystals. A hanging drops that mimicking the crystallization condition without the
107
target protein did not yield any salt crystal. Besides, salts MgCl2 and NaCl possessed high
solubility even at 4 °C and the precipitant concentration (7.5% (w/v) PEG3350) was rather
low.
4.1.5 Perspective
In this work, a purification protocol for ERα DBD-LBD was established. The preliminary
crystallogenesis of ERα DBD-LBD in complex with EREs was performed and only tiny
needle crystals were obtained. In the future, more crystallization conditions will be used to
grow high-quality crystals. If the crystal structure of ERα DBD-LBD in complex with
EREs is obtained, how ERα DBD and LBD interact with each other and function as a
whole will be exploited in depth. Moreover, the functional experiments based on the crystal
structure will be designed, such as single point mutations of certain amino acids which may
have significant roles in DBD-LDB dimerization, EREs recognition and coregulator
binding. The co-crystallization of ERα DBD-LBD with its partner proteins will be carried
out in the future studies. The partner proteins of ERα involved in the important functions in
breast cancer will be chosen as the candidates, such as FoxA1 or nm23-h1 29; 30; 31; 32; 33; 34
.
4.1.6 Acknowledgements
We thank Dr. Jiong Chen for purchasing the human full-length ERα plasmid from
Genecopoeia (Shanghai, China). We thank Dr. Kathryn Leake and Dr. Preyesh Stephen for
the revision of the manuscript. Bo Zhang thanks China Scholarship Council (CSC) for
supporting his graduate study with a national scholarship.
108
4.1.7 References
1. Heldring, N., Pike, A., Andersson, S., Matthews, J., Cheng, G., Hartman, J.,
Tujague, M., Strom, A., Treuter, E., Warner, M. & Gustafsson, J. A. (2007).
Estrogen receptors: how do they signal and what are their targets. Physiol Rev 87,
905-31.
2. Schwabe, J. W., Neuhaus, D. & Rhodes, D. (1990). Solution structure of the DNA-
binding domain of the oestrogen receptor. Nature 348, 458-61.
3. Schwabe, J. W., Chapman, L., Finch, J. T. & Rhodes, D. (1993). The crystal
structure of the estrogen receptor DNA-binding domain bound to DNA: how
receptors discriminate between their response elements. Cell 75, 567-78.
4. Schwabe, J. W., Chapman, L., Finch, J. T., Rhodes, D. & Neuhaus, D. (1993). DNA
recognition by the oestrogen receptor: from solution to the crystal. Structure 1, 187-
204.
5. Brzozowski, A. M., Pike, A. C., Dauter, Z., Hubbard, R. E., Bonn, T., Engstrom, O.,
Ohman, L., Greene, G. L., Gustafsson, J. A. & Carlquist, M. (1997). Molecular
basis of agonism and antagonism in the oestrogen receptor. Nature 389, 753-8.
6. Shiau, A. K., Barstad, D., Loria, P. M., Cheng, L., Kushner, P. J., Agard, D. A. &
Greene, G. L. (1998). The structural basis of estrogen receptor/coactivator
recognition and the antagonism of this interaction by tamoxifen. Cell 95, 927-37.
7. Tanenbaum, D. M., Wang, Y., Williams, S. P. & Sigler, P. B. (1998).
Crystallographic comparison of the estrogen and progesterone receptor's ligand
binding domains. Proc Natl Acad Sci U S A 95, 5998-6003.
8. Ascenzi, P., Bocedi, A. & Marino, M. (2006). Structure-function relationship of
estrogen receptor alpha and beta: impact on human health. Mol Aspects Med 27,
299-402.
9. Luisi, B. F., Xu, W. X., Otwinowski, Z., Freedman, L. P., Yamamoto, K. R. &
Sigler, P. B. (1991). Crystallographic analysis of the interaction of the
glucocorticoid receptor with DNA. Nature 352, 497-505.
10. Chen, Y. & Young, M. A. (2010). Structure of a thyroid hormone receptor DNA-
binding domain homodimer bound to an inverted palindrome DNA response
element. Mol Endocrinol 24, 1650-64.
109
11. Gewirth, D. T. & Sigler, P. B. (1995). The basis for half-site specificity explored
through a non-cognate steroid receptor-DNA complex. Nat Struct Biol 2, 386-94.
12. Rastinejad, F., Perlmann, T., Evans, R. M. & Sigler, P. B. (1995). Structural
determinants of nuclear receptor assembly on DNA direct repeats. Nature 375, 203-
11.
13. Williams, S. P. & Sigler, P. B. (1998). Atomic structure of progesterone complexed
with its receptor. Nature 393, 392-6.
14. Zhao, Q., Chasse, S. A., Devarakonda, S., Sierk, M. L., Ahvazi, B. & Rastinejad, F.
(2000). Structural basis of RXR-DNA interactions. J Mol Biol 296, 509-20.
15. Meijsing, S. H., Pufall, M. A., So, A. Y., Bates, D. L., Chen, L. & Yamamoto, K. R.
(2009). DNA binding site sequence directs glucocorticoid receptor structure and
activity. Science 324, 407-10.
16. Joachimiak, A. & Sigler, P. B. (1991). Crystallization of protein-DNA complexes.
Methods Enzymol 208, 82-99.
17. Gangloff, M., Ruff, M., Eiler, S., Duclaud, S., Wurtz, J. M. & Moras, D. (2001).
Crystal structure of a mutant hERalpha ligand-binding domain reveals key
structural features for the mechanism of partial agonism. J Biol Chem 276, 15059-
65.
18. Eiler, S., Gangloff, M., Duclaud, S., Moras, D. & Ruff, M. (2001). Overexpression,
purification, and crystal structure of native ER alpha LBD. Protein Expr Purif 22,
165-73.
19. Cura, V., Gangloff, M., Eiler, S., Moras, D. & Ruff, M. (2008). Cleaved thioredoxin
fusion protein enables the crystallization of poorly soluble ERalpha in complex with
synthetic ligands. Acta Crystallogr Sect F Struct Biol Cryst Commun 64, 54-7.
20. Huang, P., Chandra, V. & Rastinejad, F. (2010). Structural overview of the nuclear
receptor superfamily: insights into physiology and therapeutics. Annu Rev Physiol
72, 247-72.
21. Chandra, V., Huang, P., Hamuro, Y., Raghuram, S., Wang, Y., Burris, T. P. &
Rastinejad, F. (2008). Structure of the intact PPAR-gamma-RXR-alpha nuclear
receptor complex on DNA. Nature 456, 350-356.
110
22. Figueira, A. C., Lima, L. M., Lima, L. H., Ranzani, A. T., Mule Gdos, S. &
Polikarpov, I. (2010). Recognition by the thyroid hormone receptor of canonical
DNA response elements. Biochemistry 49, 893-904.
23. Lefstin, J. A., Thomas, J. R. & Yamamoto, K. R. (1994). Influence of a steroid
receptor DNA-binding domain on transcriptional regulatory functions. Genes Dev 8,
2842-56.
24. Gronemeyer, H. & Bourguet, W. (2009). Allosteric effects govern nuclear receptor
action: DNA appears as a player. Sci Signal 2, pe34.
25. Joachimiak, A. & Sigler, P. B. (1991). Crystallization of Protein-DNA Complexes.
Methods in Enzymology 208, 82-99.
26. Schultz, S. C., Shields, G. C. & Steitz, T. A. (1990). Crystallization of Escherichia
coli catabolite gene activator protein with its DNA binding site. The use of modular
DNA. J Mol Biol 213, 159-66.
27. Cramer, P. & Muller, C. W. (1997). Engineering of diffraction-quality crystals of
the NF-kappaB P52 homodimer:DNA complex. FEBS Lett 405, 373-7.
28. Ethayathulla, A. S., Tse, P. W., Monti, P., Nguyen, S., Inga, A., Fronza, G. &
Viadiu, H. (2012). Structure of p73 DNA-binding domain tetramer modulates p73
transactivation. Proc Natl Acad Sci U S A 109, 6066-71.
29. Laganiere, J., Deblois, G., Lefebvre, C., Bataille, A. R., Robert, F. & Giguere, V.
(2005). From the Cover: Location analysis of estrogen receptor alpha target
promoters reveals that FOXA1 defines a domain of the estrogen response. Proc Natl
Acad Sci U S A 102, 11651-6.
30. Carroll, J. S., Liu, X. S., Brodsky, A. S., Li, W., Meyer, C. A., Szary, A. J.,
Eeckhoute, J., Shao, W., Hestermann, E. V., Geistlinger, T. R., Fox, E. A., Silver, P.
A. & Brown, M. (2005). Chromosome-wide mapping of estrogen receptor binding
reveals long-range regulation requiring the forkhead protein FoxA1. Cell 122, 33-43.
31. Lupien, M., Eeckhoute, J., Meyer, C. A., Wang, Q., Zhang, Y., Li, W., Carroll, J. S.,
Liu, X. S. & Brown, M. (2008). FoxA1 translates epigenetic signatures into
enhancer-driven lineage-specific transcription. Cell 132, 958-70.
111
32. Hurtado, A., Holmes, K. A., Ross-Innes, C. S., Schmidt, D. & Carroll, J. S. (2011).
FOXA1 is a key determinant of estrogen receptor function and endocrine response.
Nat Genet 43, 27-33.
33. Curtis, C. D., Likhite, V. S., McLeod, I. X., Yates, J. R. & Nardulli, A. M. (2007).
Interaction of the tumor metastasis suppressor nonmetastatic protein 23 homologue
H1 and estrogen receptor alpha alters estrogen-responsive gene expression. Cancer
Res 67, 10600-7.
34. Schultz-Norton, J. R., Ziegler, Y. S. & Nardulli, A. M. (2011). ERalpha-associated
protein networks. Trends Endocrinol Metab 22, 124-9.
112
Figure 4.1.1 The constructions of Human ERα DBD-LBD recombinant plasmids
In (A) and (B), Lanes 1 and 2 are PCR results of two different clones of the pET-28a(+)
recombinant plasmids encoding ERα 179-554aa and 179-595aa, respectively; lanes 3
and 4 are the corresponding recombinant plasmids digested by two restriction enzymes
(BamHI and XhoI).
113
Figure 4.1.2 The verification of ERα DBD-LBD expression in Rosetta2 (DE3)
cells
(A) PCR results of two different Rosetta2 (DE3) clones containing ERα 179-554aa and
179-595aa encoding plasmids, respectively, lanes 1 and 2 encoding ERα 179-554aa and
lanes 3 and 4 encoding ERα 179-595aa; (B) ERα 179-554aa and 179-595aa expression
induced by IPTG in Rosetta2 (DE3) cells, lanes 1 and 2 are none-induced and induced
results of ERα 179-554aa, lanes 3 and 4 are none-induced and induced results of ERα
179-595aa.
114
Figure 4.1.3 Expression results of ERα DBD-LBD (179-595aa) in Rosetta2 (DE3)
cells
(A) and (B) are ERα 179-595aa expression in 18 °C and 25 °C, respectively. Lane 1 is the
total protein in the cells, lane 2 is protein in the supernatant and lane 3 is protein in the
precipitate.
115
Figure 4.1.4 Purification results of ERα DBD-LBD (179-595aa)
(A) Lanes 1 and 2 are the peak fractions of ERα 179-595aa eluted from the nickel column,
Lanes 3 and 4 are the peak fractions of ERα 179-595aa eluted from the gel filtration
column and the purity is above 95%; (B) two purified samples of ERα 179-595aa are
verified by Western blot.
116
Figure 4.1.5 Preliminary crystallogenesis of ERα DBD-LBD (179-554aa)
The needle crystals were obtained at 4 °C in a crystallization condition containing 7.5%
(w/v) PEG3350, 0.1 M MES buffer (pH 7.0), 0.1 M MgCl2 and 0.2 M NaCl.
117
4.2 A SIMPLE AND EFFICIENT PURIFICATION METHOD FOR
HUMAN ESTROGEN RECEPTOR ALPHA LBD
A simple and efficient purification method for human estrogen receptor
alpha LBD
Bo Zhang 1, 2
, Jean-François Thériault 1, Dao-Wei Zhu
1, Sheng-Xiang Lin
1, §
1 Laboratory of Molecular Endocrinology and Oncology, Centre Hospitalier Universitaire
(CHU) de Quebec Research Center (CHUL) and Laval University, Québec City, Québec,
G1V4G2, Canada
2 Key Laboratory for Space Bioscience & Biotechnology, Institute of Special
Environmental Biophysics, School of Life Sciences, Northwestern Polytechnical University,
Xi’an, P. R. China, 710072
§ Corresponding Author: S.-X. Lin, CHUL Research Center, 2705 Boul. Laurier, Québec
City, QC, G1V4G2, Canada; Tel.: +1 418 654 2296
E-mail: [email protected]
Shortened title: an efficient purification method for human ERα LBD
118
4.2.1 Abstract
Human estrogen receptor alpha (ERα), activated by the binding of 17β-estradiol (E2),
exerts its essential effects on sexual development and reproductive functions. It has been
well established that the ligand binding domain (LBD) of ERα is sensitive to oxidation and
aggregation. Several methods have been developed to purify ERα LBD, such as
carboxymethylations or mutations of reactive cysteine residues, denaturation and
renaturation, introducing high concentration of reducing agent or fusion protein. Here, a
novel simple and efficient purification method for ERα LBD with a mutation of C530A
was reported. The target protein was expressed in E. coli BL21(DE3) cells. After the cell
pellets were lysed and centrifuged, the precipitate was used for purification. Several
detergents such as Triton X-100 and β-DDM (dodecyl-β-D-maltoside) were selected to
dissolve the precipitate and above 70% purity of the target protein was reached by the
treatment with detergents. Moreover, using a combination of detergents (Triton X-100 and
β-OG (β-Octyl glucoside)), one step of the purification by the nickel column could yield the
homogeneous and highly purified protein.
Keywords: estrogen receptor alpha (ERα), the ligand binding domain (LBD), detergent,
precipitate, purification.
119
4.2.2 Introduction
Nuclear receptors (NRs) act as transcription factors through binding a variety of
physiological hormones to regulate the transcription of specific genes, which play critical
roles in numerous physiological functions such as reproductive health and embryonic
development 1; 2
. Defined as a member of the NRs superfamily, estrogen receptor alpha
(ERα) is activated by the binding of 17β-estradiol (E2) to the ligand binding domain (LBD)
of ERα. The liganded ERα targets specific promoters or enhancers of genes through its
DNA binding domain (DBD) binding to estrogen response elements (EREs) and exerts its
effects on sexual development and reproductive functions 3; 4
. ERα LBD can bind a variety
of ligands, and part of its ligands act as agonists while others function as antagonists.
Through binding to agonists, the conformation of ERα LBD helix12 is rearranged, which
makes ERα LBD qualified to recruit coactivators such as steroid receptor coactivator 1
(SRC-1) 5; 6
. In contrast, through binding to antagonists, ERα LBD possesses the ability to
recruit corepressors such as nuclear receptor corepressor (NcoR) 1; 7
.
Although the crystal structures of ERα LBD in complex with agonists and antagonists have
been reported 5; 6; 8
, the purification processes of ERα LBD are full of challenges. There are
four cysteine residues in ERα LBD, and among them three residues (Cys381, Cys417 and
Cys530) are exposed to solvent and are sensitive to oxidation 9. Moreover, ERα LBD is
recognized by its hydrophobic character and is unstable without binding its ligands, which
makes it prone to aggregation. To date, several methods have been established to solve the
difficulties in purification. Initially, carboxymethylation of three reactive cysteine residues
in ERα LBD was successfully used to purify and crystallize this protein 5; 6; 9
. In addition,
denaturation and renaturation of ERα LBD was used to accomplish purification 8. The triple
cysteine to serine mutagenesis of ERα LBD was also introduced to reduce the difficulties of
purification 10
. Eiler and coworkers obtained the purified native form ERα LBD by using
high concentration of reducing agent to avoid the oxidation of cysteine residues during the
purification process 11
. In addition, Cura and coworkers developed a cleavable fusion
protein to increase the solubility of the target protein, and successfully purified ERα LBD 12
.
In this study, the residue Cys530 in ERα LBD was initially mutated to alanine. ERα LBD
Cys530 was the most reactive residue and could form the intermolecular disulfide bond
120
without high concentration of reducing agent 8. During the purification process of ERα
LBD, even under the optimized expression conditions in E. coli BL21(DE3) cells, the
major part of the target protein was predominantly kept in the precipitate. The soluble
portion in the supernatant was rather poor. This impelled us to develop a simple and
efficient purification method to obtain ERα LBD from the precipitate by using a
combination of different detergents.
4.2.3 Methods
4.2.3.1 Site-directed mutagenesis of ERα LBD C530A
The DNA fragment encoding human ERα LBD (297-554aa (amino acids)) was cloned into
pET-28a(+) vector. Using the recombinant vector as the template, the single point mutation
of ERα LBD C530A was performed by following the QuikChange Lightning Kit (Agilent
Technologies) protocol with 5’-CTGTACAGCATGAAGGCCAAGAACGTGGTGCC-3’
as forward primer and the result was verified by sequencing.
4.2.3.2 Protein expression and purification
Human ERα LBD with a mutation of C530A was expressed in E. coli BL21(DE3) cells.
The cells were grown at 37°C for 3 hours until OD600 reached 0.6, and then cells were
induced with 0.2 mM IPTG at 18°C in the presence of 10 μM 17β-estradiol overnight,
harvested and lysed in buffer A (50 mM Tris-HCl (pH 8.0), 10 mM imidazole, 200 mM
NaCl, 10% glycerol, 20 mM β-mercaptoethanol, 1 mM PMSF and 10 μM 17β-estradiol)
with the addition of 1 mg/ml lysozyme and 1 μg/ml each of protease inhibitors (leupeptin,
chymostatin, antipain, aprotinin, pepstatin A and benzamidin). After sonication and
centrifugation, the supernatant was discarded. The precipitate was resuspended in buffer A
with 0.4% Triton X-100 and protease inhibitors, and was slowly agitated via a magnetic
stirrer at 4°C overnight. After centrifugation for the second time, the supernatant was
collected and loaded onto the nickel column pre-equilibrated in buffer A with 0.2% Triton
X-100 and 0.1% β-OG. After incubation at 4°C for 3 hours, the nickel column was washed
with 15 column volumes (CV) buffer A containing 0.2% Triton X-100 and 0.1% β-OG, and
then washed with 15 CV buffer A containing 30 mM imidazole, 0.1% Triton X-100, 0.1%
121
β-OG and another step of 15 CV buffer A containing 30 mM imidazole and 0.1% β-OG.
Next, the target protein was eluted with 10 CV buffer A containing 200 mM imidazole and
0.1% β-OG. The eluted fractions were concentrated by a centrifugal filter with a 10 kDa
molecular weight cutoff and the buffer was exchanged to 50 mM Tris-HCl (pH 8.0), 100
mM NaCl, 5% glycerol, 5 mM DTT, 0.5 M NDSB-201 (non detergent sulfobetaines), 10
μM 17β-estradiol and 0.1% β-OG by three rounds of dilution and concentration. The purity
of the concentrated ERα LBD was estimated by SDS-PAGE and above 98%. The protein
concentration was determined as approximately 9.1 mg/ml using the Bradford method.
4.2.3.3 Solubility test
The E.coli cells containing the ERα LBD C530A recombinant plasmids were grown in 200
ml LB (Lysogeny broth) medium at 37°C for 2.5 hours until OD600 reached 0.6. Next, the
E.coli cells were induced by 0.2 mM IPTG at 18°C for 14-16 hours in the presence of 10
μM 17β-estradiol. The cell pellets were harvested, resuspended in 10 ml buffer A, sonicated
and centrifuged. Supernatant was discarded and precipitate was resuspended in 10 ml
buffer A. Each solubility test required 0.5 ml resuspended sample. 0.4% (w/v) each of
Triton X-100, C12E8 (octaethylene glycol monododecyl ether), β-DDM (dodecyl-β-D-
maltoside), β-OG (β-octyl glucoside) and Emulgen913 was added to the 0.5 ml sample,
respectively, and samples were slowly agitated overnight at 4°C. After samples were
centrifuged, the supernatant and the precipitate were checked by SDS-PAGE.
4.2.4 Results and discussion
4.2.4.1 Expression and solubility test of ERα LBD
The expression of the ERα LBD C530A mutant was induced with 0.2 mM IPTG at 18°C
for 14-16 hours in the presence of 10 μM 17β-estradiol in E.coli BL21 (DE3) cells. The cell
pellets were harvested and lysed in buffer A with 1 mg/ml lysozyme and 1 μg/ml each of
protease inhibitors (leupeptin, chymostatin, antipain, aprotinin, pepstatin A and
benzamidin). After sonication and centrifugation, the target protein predominantly existed
in the precipitate (Figure 4.2.1). Then, 0.4% (w/v) each of Triton X-100, Tween-20, C12E8,
β-DDM, β-OG and Emulgen913 was applied to the solubility test. The results showed that
122
Triton X-100, C12E8, β-DDM and Emulgen913 considerably improved the target protein to
be present in the supernatant. Particularly, above 70% purity was achieved by the treatment
with Triton X-100, C12E8 and Emulgen913 (Figure 4.2.2).
4.2.4.2 Purification of ERα LBD
Hereafter, the precipitate was used for the purification of ERα LBD. The precipitate was
resuspended again in buffer A containing 0.4% Triton X-100 and was then slowly agitated
at 4°C overnight. After centrifugation, the supernatant was obtained, filtered and loaded
onto the nickel column pre-equilibrated in buffer A with 0.2% Triton X-100 and 0.045% β-
DDM. After incubation at 4°C for 3 hours, the target protein was eluted with buffer A
containing 200 mM imidazole and 0.045% β-DDM. However, the target protein began to
aggregate soon after the elution from the nickel column. Therefore, 0.03% C12E8, 0.035%
Emulgen913 and 0.1% β-OG were tested to replace 0.045% β-DDM, respectively. 0.1% β-
OG was found to significantly relieve aggregation. Additionally, 0.5 M NDSB-201 was
also added to buffer A to improve the solubility of the target protein. Following the
procedures mentioned in Methods, the eluted fractions in buffer A containing 200 mM
imidazole, 0.1% β-OG and 0.5 M NDSB-201 were concentrated and then the buffer was
exchanged to 50 mM Tris-HCl (pH 8.0), 100 mM NaCl, 5% glycerol, 5 mM DTT, 0.1% β-
OG, 0.5 M NDSB-201 and 10 μM 17β-estradiol. This protocol used one step of the nickel
column to complete the purification. The protein concentration reached 9.1 mg/ml and the
purity was estimated to be above 98% by SDS-PAGE (Figure 4.2.3). Although further
purification by a Sephacryl S-200 gel-filtration column could improve the result, this step
was not necessary. A unique absorption peak during the gel filtration step indicated that the
target protein purified by the nickel column was rather homogeneous and the oligomeric
potential of ERα LBD was not observed. In addition, following this protocol, 25-30 mg of
ERα LBD could be obtained from a liter of the E.coli cells. This protocol was also
appropriate for the purification of ERα LBD in its native form (without the C530A
mutation). However, high concentration of the reducing agent was required for this task 11
.
123
4.2.5 Acknowledgements
The authors wish to thank Dr. Jiong Chen for purchasing the human full-length ERα
plasmid from Genecopoeia (Shanghai, China). The authors thank Dr. Kathryn Leake and
Dr. Preyesh Stephen for the revision of the manuscript. Bo Zhang appreciates China
Scholarship Council (CSC) for providing him a national scholarship.
124
4.2.6 References
1. Huang, P., Chandra, V. & Rastinejad, F. (2010). Structural overview of the nuclear
receptor superfamily: insights into physiology and therapeutics. Annu Rev Physiol
72, 247-72.
2. Olefsky, J. M. (2001). Nuclear receptor minireview series. J Biol Chem 276, 36863-
4.
3. Korach, K. S. (1994). Insights from the study of animals lacking functional estrogen
receptor. Science 266, 1524-7.
4. Heldring, N., Pike, A., Andersson, S., Matthews, J., Cheng, G., Hartman, J.,
Tujague, M., Strom, A., Treuter, E., Warner, M. & Gustafsson, J. A. (2007).
Estrogen receptors: how do they signal and what are their targets. Physiol Rev 87,
905-31.
5. Brzozowski, A. M., Pike, A. C., Dauter, Z., Hubbard, R. E., Bonn, T., Engstrom, O.,
Ohman, L., Greene, G. L., Gustafsson, J. A. & Carlquist, M. (1997). Molecular
basis of agonism and antagonism in the oestrogen receptor. Nature 389, 753-8.
6. Shiau, A. K., Barstad, D., Loria, P. M., Cheng, L., Kushner, P. J., Agard, D. A. &
Greene, G. L. (1998). The structural basis of estrogen receptor/coactivator
recognition and the antagonism of this interaction by tamoxifen. Cell 95, 927-37.
7. Bain, D. L., Heneghan, A. F., Connaghan-Jones, K. D. & Miura, M. T. (2007).
Nuclear receptor structure: implications for function. Annu Rev Physiol 69, 201-20.
8. Tanenbaum, D. M., Wang, Y., Williams, S. P. & Sigler, P. B. (1998).
Crystallographic comparison of the estrogen and progesterone receptor's ligand
binding domains. Proc Natl Acad Sci U S A 95, 5998-6003.
9. Hegy, G. B., Shackleton, C. H., Carlquist, M., Bonn, T., Engstrom, O., Sjoholm, P.
& Witkowska, H. E. (1996). Carboxymethylation of the human estrogen receptor
ligand-binding domain-estradiol complex: HPLC/ESMS peptide mapping shows
that cysteine 447 does not react with iodoacetic acid. Steroids 61, 367-73.
10. Gangloff, M., Ruff, M., Eiler, S., Duclaud, S., Wurtz, J. M. & Moras, D. (2001).
Crystal structure of a mutant hERalpha ligand-binding domain reveals key
structural features for the mechanism of partial agonism. J Biol Chem 276, 15059-
65.
125
11. Eiler, S., Gangloff, M., Duclaud, S., Moras, D. & Ruff, M. (2001). Overexpression,
purification, and crystal structure of native ER alpha LBD. Protein Expr Purif 22,
165-73.
12. Cura, V., Gangloff, M., Eiler, S., Moras, D. & Ruff, M. (2008). Cleaved thioredoxin
fusion protein enables the crystallization of poorly soluble ERalpha in complex with
synthetic ligands. Acta Crystallogr Sect F Struct Biol Cryst Commun 64, 54-7.
126
Figure 4.2.1 Expression result of ERα LBD
The E. coli cell pellets were lysed in buffer, sonicated and centrifuged. The total protein,
the supernatant and the precipitate are shown in lanes 1, 2 and 3, respectively.
127
Figure 4.2.2 Solubility test of ERα LBD
The E.coli cell pellets were lysed in buffer, sonicated and centrifuged. The supernatant
was discarded and the precipitate was preserved. The precipitate was resuspended and
treated with 0.4% (w/v) each of Triton X-100, C12E8, β-DDM, Emulgen913,
respectively; lanes 1, 3, 5 and 7 are proteins remained in the precipitate and lanes 2, 4, 6
and 8 are proteins dissolved from the precipitate.
128
Figure 4.2.3 Purification result of ERα LBD
Lanes 1 and 2 are the peak fractions of ERα LBD eluted from the nickel column, the purity
of ERα LBD is above 98%.
129
CHAPTER 5 CONCLUSIONS
130
Human 3-alpha hydroxysteroid dehydrogenase type 3 (3α-HSD3) has an essential role to
inactivate the most potent androgen 5α-dihydrotestosterone (5α-DHT). Meanwhile, 5α-
DHT has been shown to reduce breast cancer cells growth and the role of 3α-HSD3 in
breast cancer is short of investigations. The goal of my study is to investigate the structure-
function relationship of 3α-HSD3 in complex with various steroids, and to further
investigate the potential role of 3α-HSD3 in breast cancer cells. In addition, estrogen
receptor alpha (ERα) controls sexual development and reproductive functions. Another goal
of my study is to purify the ERα fragment including its DNA binding domain and ligand
binding domain (DBD-LBD), and try to obtain the crystal structure of ERα DBD-LBD in
complex with estrogen response elements (EREs). The main accomplishments are as
following:
(1) To understand the role of residue 54 in the steroid binding and discrimination, the
Val54-to-Leu54 (V54L) mutation in human 3α-HSD3 has been created. We report two
crystal structures of the 3α-HSD3·NADP+·Progesterone complex and the 3α-HSD3
V54L·NADP+·progesterone complex. These crystal structures show that progesterone in
the wild type enzyme possesses two different binding modes, which indicates the steroid
binding pocket possessing considerable flexibility to accommodate different orientations of
a steroid. However, in the mutant enzyme, the bulky side chain of Leu54 significantly
confines the spatial movement of the steroid and thus only one orientation presents in the
steroid binding pocket. Moreover, we report that the V54L mutation in 3α-HSD3
significantly decreases its 5α-DHT inactivation ability and this mutation enhances the 20-
alpha hydroxysteroid dehydrogenase (20α-HSD) activity to catalyze progesterone.
(2) We report the crystal structure of the 3α-HSD3·NADP+·A-dione/epi-ADT complex,
which is obtained by co-crystallization with 5α-DHT. Although 5α-DHT was introduced
during the crystallization, the oxidoreduction of 5α-DHT occurred. A-dione and epi-ADT
were identified to be located in the steroid binding sites of two monomers (monomer A and
B) in a crystal asymmetric unit, respectively. An overlay of monomer A and B shows that
A-dione and epi-ADT are oriented upside down and flipped to each other, which provides
the structural clues of 5α-DHT alternative binding within the enzyme to yield different
products. Moreover, using a crystallization condition without acetate ion, we report the
131
crystal structure of the 3α-HSD3·NADP+·4-dione complex. In addition, using specific
siRNA to knock down 3α-HSD3 expression in MCF7 breast cancer cells, 5α-DHT
concentration increased while the cell growth was suppressed.
(3) We set up an expression and purification protocol of ERα DBD-LBD. Preliminary
crystallogenesis of ERα DBD-LBD in complex with estrogen response elements (EREs) is
carried out. This study provides the basic knowledge to facilitate the acquisition of the fine
crystals for ERα DBD-LBD in complex with EREs.
(4) We report a simple and efficient purification method for human ERα LBD.
5.1 STRUCTURE-FUNCTION STUDY OF HUMAN 3ΑLPHA-HSD3
SINGLE POINT MUTATION V54L ENHANCING THE 20ΑLPHA-HSD
ACTIVITY
Human 3α-HSD3 plays an essential role to inactivate androgen 5α-DHT, while human 20α-
HSD is responsible for inactivation of progesterone. However, there is only one amino acid
difference (residue 54) between the steroid binding pockets of 3α-HSD3 and 20α-HSD. By
combining mutagenesis, X-ray crystallography and enzyme kinetics study, we explore the
role of residue 54 in the steroid binding and discrimination.
We report the crystal structure of the 3α-HSD3·NADP+·Progesterone complex. There are
two monomers (monomer A and B) in a crystal asymmetric unit. In monomer A, the α-face
of progesterone interacts with Val54 and Val128 and the steroid C18 and C19 methyl
groups pointing toward Trp227. However, in monomer B, the steroid α-face is in stacking
with Trp227 and the two methyl groups of the steroid are pointing toward Tyr55. When
two monomers are superimposed, it shows that loop A fluctuates notably compared with
loop B and loop C, and two steroids in the cavities could not overlap each other and their
orientations have a difference of ~105° rotation around the long axis of C10-C17. The side
chains of His222 and Leu308 flip 180° and the side chain of Leu306 owns alternative
conformations. These results demonstrate that the steroid binding pocket of 3α-HSD3
possesses considerable flexibility to accommodate different orientations of a steroid.
132
We also report the crystal structure of the 3α-HSD3 V54L·NADP+·progesterone complex.
An overlay of monomer A and B in the crystal asymmetric unit shows high similarity for
their overall structures, and the orientations of two steroids overlap each other quite well.
The α-faces of both steroids interact with Leu54 and Val128, and their β-faces interact with
the Trp227 indole group. The bulky side chain of Leu54 in the mutant enzyme is
outstretching toward the steroid and obviously generates a steric hindrance to restrict the
steroid rotation. Moreover, steroids in the mutant enzyme possess relatively lower B-factors
in monomer A and B (23.3/27.6 Å2) than that in the wild type enzyme (37.7/34.4 Å
2),
which implies the V54L mutation has a role of stabilization for progesterone. Therefore, the
V54L mutation significantly restricts the spatial movement of the steroid and eliminates
multiple orientations which are allowed in the wild type enzyme.
To further understand the steroid discrimination by human 3α-HSD3 and its V54L mutant,
the kinetic study has been carried out. The V54L mutation in 3α-HSD3 significantly
decreases its 3α-reductase activity and enhances its 20α-reductase activity. For 5α-DHT
reduction, the kinetic parameters for the wild type enzyme (Km = 2.18 μM, kcat = 3.67 min-1
and kcat/Km = 1.68 min-1
μM-1
) and the mutant enzyme (Km = 71.03 μM, kcat = 6.92 min-1
and
kcat/Km = 0.10 min-1
μM-1
) indicate that the 5α-DHT reduction ability is significantly
decreased in the mutant enzyme. While for progesterone reduction, the kinetic parameters
for the wild type enzyme (Km = 0.84 μM, kcat = 0.21 min-1
and kcat/Km = 0.25 min-1
μM-1
)
and the mutant enzyme (Km = 2.13 μM, kcat = 2.35 min-1
and kcat/Km = 1.10 min-1
μM-1
)
indicate that the wild type enzyme possesses a weak activity and the mutant enzyme shows
a considerable 20α-reduction activity. The results imply that, for those homologous
enzymes, only one residue alteration at the substrate binding pocket is enough to transform
the substrate specificity for the enzyme.
5.2 STRUCTURAL CLUES OF 5ΑLPHA-DHT ALTERNATIVE BINDING
WITHIN HUMAN 3ΑLPHA-HSD3 AND DOWN-REGULATION OF
3ΑLPHA-HSD3 DECREASING BREAST CANCER CELL GROWTH
Androgen 5α-DHT has been shown to prevent breast cancer cells growth. In human, 3α-
HSD3 functions as the 3-ketosteroid reductase to inactivate 5α-DHT in cellular
133
environment. However, the role of 3α-HSD3 in breast cancer cells is short of investigations.
In this study, we try to obtain the crystal structure of 3α-HSD3 in complex with 5α-DHT. In
addition, using specific siRNA to knockdown 3α-HSD3 expression in breast cancer cells
(MCF7), the impacts of 3α-HSD3 expression on 5α-DHT concentration and cell
proliferation are investigated.
A high-resolution crystal structure of human 3α-HSD3·NADP+·A-dione/epi-ADT complex
is obtained by co-crystallization with 5α-DHT in presence of NADP+. Although 5α-DHT is
introduced during the crystallization, the oxidoreduction of 5α-DHT occurs and generates a
mixture of steroids. A-dione and epi-ADT are identified to be located in the cavities of two
monomers (monomer A and B) in a crystal asymmetric unit, respectively. In monomer A,
the D-ring of A-dione is oriented toward the nicotinamide ring. The α-face of A-dione
interacts with the side chain of Val54, Trp86 and Val128. Its β-face mainly interacts with
the indole ring of Trp227, and the steroid C18 and C19 methyl groups are pointing toward
Trp227. In monomer B, the A-ring of epi-ADT is pointing toward the nicotinamide ring.
The α-face of epi-ADT is stacking with the indole ring of Trp227, and the steroid C18 and
C19 methyl groups are pointing toward Val54 and Tyr55. When monomer A and B are
superimposed, two steroids are oriented upside down to each other, and the planes of two
steroids are flipped about 145° around the long axis of C3-C17. In both monomers,
fluctuation in loop A is prominent. The side chains of Val128, Ile129 and Leu306 display
apparent movement to consort with steroids. The different orientations of A-dione and epi-
ADT provide the structural clues of 5α-DHT having the alternative binding modes in the
cavity of the enzyme to generate different products. The alternative binding modes of
steroids in the enzyme originate from the pseudo self-symmetry property of androgens and
the flexibility of the steroid binding pocket.
The crystal structure of human 3α-HSD3·NADP+·4-dione complex is obtained by co-
crystallization with Testo in the presence of NADP+. During the crystallization process, the
oxidation of Testo occurs and 4-dione is identified to be located in the steroid binding
pockets of monomer A and B in a crystal asymmetric unit. When superimposing monomer
A and B, the orientation and conformation of 4-dione are quite similar to each other. Loop
A still displays its flexibility. The A-ring of 4-dione is pointing toward the nicotinamide
134
ring. The α-face of 4-dione interacts with the side chain of Trp227, and the C18 and C19
methyl groups of 4-dione are pointing toward the side chain of His117. Compared with the
orientation of Testo in the reported 3α-HSD3·NADP+·Testo/acetate complex, the
orientation of 4-dione in the 3α-HSD3·NADP+·4-dione complex generates ~45° rotation
around its C3-C17 long axis. Meanwhile, the steroid goes deeper into the cavity of the
enzyme. The acetate molecule in the Testo/acetate complex, which is originated from the
crystallization condition, occupies the active site of the enzyme and distorts the actual
steroid binding conformation. However, using a crystallization condition without the
acetate molecule, the steroid binding conformation of 4-dione was more reasonable and less
distorted.
In addition, the 3α-HSD3 expression is knocked down by specific siRNA in MCF7 cells,
and a relative elevation of 5α-DHT level is detected by using ELISA assay. Meanwhile, in
the presence of 5α-DHT, suppression of 3α-HSD3 expression by specific siRNA leads to a
decrease of MCF7 cell growth, which can be speculated that the suppressed expression of
3α-HSD3 strengthens the antiproliferative effect of 5α-DHT in MCF7 cells. It is
noteworthy that suppression of 17β-HSD1 expression is reported to increase 5α-DHT level
in T47D cells, which shows an antiproliferative effect. However, compared with 5α-DHT
inactivation ability of 17β-HSD1, 3α-HSD3 possesses a significant higher activity to
convert 5α-DHT, which implies that 3α-HSD3 may undertake a more important role than
17β-HSD1 to inactivate 5α-DHT in breast cancer cells.
5.3 PURIFICATION AND PRELIMINARY CRYSTALLOGENESIS OF
HUMAN ESTROGEN RECEPTOR ALPHA DBD-LBD
ERα plays important physiological functions in human such as controlling sexual
development and reproductive functions. However, due to the difficulties in protein
purification and crystallization, the full-length ERα structure remains an unfulfilled task. In
this study, we set up an expression and purification protocol of ERα fragment containing its
DNA binding domain and ligand binding domain (DBD-LBD).
At the beginning, the recombinant plasmid encoding ERα DBD-LBD with the C530A
single point mutation was transformed into E.coli Rosetta2 (DE3) cells. The expressions of
135
the target protein were induced with different concentrations of IPTG at 37°C. However,
after sonication and centrifugation, the target protein existed mostly in the precipitant, not
in the supernatant. Several commonly used detergents were used to improve the protein
solubility, whereas these detergents had little efficacy for improving the solubility of ERα
DBD-LBD. After optimization of the expressing conditions, 25°C for 12 hours and 0.2 mM
IPTG were determined to induce the target protein to be expressed in the supernatant with
an acceptable quantity. During the purification, the target protein was prone to aggregate.
However, high salt concentration (above 400 mM NaCl) was found significantly preventing
the protein aggregation and increasing the solubility of ERα DBD-LBD. Through two steps
of purification by the nickel column and the gel filtration column, ERα DBD-LDB was
concentrated to 6.0 mg/ml and the purity was above 95 %. In addition, Western blot further
proved the target band representing ERα DBD-LBD. Preliminary crystallogenesis of ERα
DBD-LBD in complex with estrogen response elements (EREs) was carried out. This study
provided the basic knowledge to facilitate the acquisition of the fine crystals for ERα DBD-
LBD in complex with EREs.
5.4 A SIMPLE AND EFFICIENT PURIFICATION METHOD FOR
HUMAN ESTROGEN RECEPTOR ALPHA LBD
ERα ligand binding domain (LBD) is sensitive to oxidation and aggregation. Previously,
several methods were developed to purify ERα LBD, such as carboxymethylation or
mutation of reactive cysteine residues, denaturation and renaturation, introducing high
concentration of reducing agents or fusion protein. Here, we reported a novel simple and
efficient purification method for human ERα LBD.
ERα LBD was induced to express in E.coli BL21 (DE3) cells with 0.2 mM IPTG at 18°C.
The cell pellets were harvested and lysed. After sonication and centrifugation, compared
with the supernatant, the target protein was found mainly existing in the precipitant. Several
detergents were selected to dissolve the precipitant. It was found that Triton X-100, C12E8,
β-DDM, Emulgen913 considerably improved the target protein to exist in the supernatant,
and above 70 % purity of the target protein has been reached by treatment with 0.4 % of
Triton X-100, C12E8 and Emulgen913. Thus, 0.4 % Triton X-100 was chosen to extract the
136
target protein from the precipitant. Furthermore, using a combination of Triton X-100 and
β-OG, the purification of ERα LBD could be fulfilled by only using the nickel column. The
protein concentration reached to 9.1 mg/ml and the purity was above 98 %. Further step of
purification by the gel filtration column could polish the purification result, but not
necessary.
5.5 FUTURE TOPICS
Although some progress has been made, more structural and functional studies need to be
carried out to further clarify the role of 3α-HSD3 in breast cancer cells. For example:
(1) Our study shows the structural clues of 5α-DHT and progesterone alternative binding
within 3α-HSD3. However, different from the productive binding orientation of the steroid
in rat 3α-HSD, steroids display the binding orientations before or after the reactions within
3α-HSD3. Therefore, the molecular dynamics simulation can be carried out to provide the
dynamic information of 3α-HSD3 utilizing the alternative binding modes of steroids to
output different products.
(2) Due to the role of the inactivation of 5α-DHT by 3α-HSD3, certain leading compounds
can be designed to inhibit 3α-HSD3. This may have an effect on increasing the 5α-DHT
concentration in breast cancer cells and decreasing the growth of breast cancer cells.
(3) It has been shown that the transcription of 3α-HSD3 is regulated by transcription factor
Nrf2 (nuclear factor erythroid-2 related factor 2). The role of Nrf2 in breast cancer cells
should be further studied. Moreover, the impact of 3α-HSD3 down-regulation by siRNA on
the gene and protein profile of breast cancer cells should be investigated. The differentially
expressed candidates that may get involved in breast cancer should be further investigated.
In addition, for human ERα DBD-LBD, more crystallization conditions and the target
protein in complex with different estrogen response elements should be attempted to obtain
high-quality crystals. The co-crystallization of ERα DBD-LBD with its partner proteins
such as FoxA1 and nm23-h1, which are closely related to breast cancer, will be another
direction of the research.
137
CHAPTER 6 REFERENCES (FOR INTRODUCTION)
138
REFERENCES
1. Poirier, D. (2010). 17beta-Hydroxysteroid dehydrogenase inhibitors: a patent
review. Expert Opin Ther Pat 20, 1123-45.
2. Griffiths, K., Morton, M. S. & Nicholson, R. I. (1997). Androgens, androgen
receptors, antiandrogens and the treatment of prostate cancer. Eur Urol 32 Suppl 3,
24-40.
3. Miller, W. L. (1988). Molecular biology of steroid hormone synthesis. Endocr Rev
9, 295-318.
4. Strauss, J. F. & Barbieri, R. L. (2009). Yen and Jaffe's reproductive endocrinology :
physiology, pathophysiology, and clinical management. 6th edit, Saunders/Elsevier,
Philadelphia, PA.
5. Labrie, F., Luu-The, V., Lin, S. X., Simard, J., Labrie, C., El-Alfy, M., Pelletier, G.
& Belanger, A. (2000). Intracrinology: role of the family of 17 beta-hydroxysteroid
dehydrogenases in human physiology and disease. J Mol Endocrinol 25, 1-16.
6. Luu-The, V. & Labrie, F. (2010). The intracrine sex steroid biosynthesis pathways.
Prog Brain Res 181, 177-92.
7. Labrie, F., Luu-The, V., Labrie, C., Belanger, A., Simard, J., Lin, S. X. & Pelletier,
G. (2003). Endocrine and intracrine sources of androgens in women: inhibition of
breast cancer and other roles of androgens and their precursor
dehydroepiandrosterone. Endocr Rev 24, 152-82.
8. Adams, J. B. & McDonald, D. (1980). Enzymic synthesis of steroid sulphates. XIII.
Isolation and properties of dehydroepiandrosterone sulphotransferase from human
foetal adrenals. Biochim Biophys Acta 615, 275-8.
9. Luu-The, V., Bernier, F. & Dufort, I. (1996). Steroid sulfotransferases. J Endocrinol
150 Suppl, S87-97.
10. Miller, W. L. & Auchus, R. J. (2011). The molecular biology, biochemistry, and
physiology of human steroidogenesis and its disorders. Endocr Rev 32, 81-151.
11. Reed, M. J., Purohit, A., Woo, L. W., Newman, S. P. & Potter, B. V. (2005).
Steroid sulfatase: molecular biology, regulation, and inhibition. Endocr Rev 26,
171-202.
139
12. Migeon, B. R., Shapiro, L. J., Norum, R. A., Mohandas, T., Axelman, J. & Dabora,
R. L. (1982). Differential expression of steroid sulphatase locus on active and
inactive human X chromosome. Nature 299, 838-40.
13. Alperin, E. S. & Shapiro, L. J. (1997). Characterization of point mutations in
patients with X-linked ichthyosis. Effects on the structure and function of the
steroid sulfatase protein. J Biol Chem 272, 20756-63.
14. Labrie, F., Luu-The, V., Lin, S. X., Labrie, C., Simard, J., Breton, R. & Belanger, A.
(1997). The key role of 17 beta-hydroxysteroid dehydrogenases in sex steroid
biology. Steroids 62, 148-58.
15. Moghrabi, N. & Andersson, S. (1998). 17beta-hydroxysteroid dehydrogenases:
physiological roles in health and disease. Trends Endocrinol Metab 9, 265-70.
16. Ghosh, D., Pletnev, V. Z., Zhu, D. W., Wawrzak, Z., Duax, W. L., Pangborn, W.,
Labrie, F. & Lin, S. X. (1995). Structure of human estrogenic 17 beta-
hydroxysteroid dehydrogenase at 2.20 A resolution. Structure 3, 503-13.
17. Peltoketo, H., Luu-The, V., Simard, J. & Adamski, J. (1999). 17beta-hydroxysteroid
dehydrogenase (HSD)/17-ketosteroid reductase (KSR) family; nomenclature and
main characteristics of the 17HSD/KSR enzymes. J Mol Endocrinol 23, 1-11.
18. Lachance, Y., Luu-The, V., Labrie, C., Simard, J., Dumont, M., de Launoit, Y.,
Guerin, S., Leblanc, G. & Labrie, F. (1990). Characterization of human 3 beta-
hydroxysteroid dehydrogenase/delta 5-delta 4-isomerase gene and its expression in
mammalian cells. J Biol Chem 265, 20469-75.
19. Lorence, M. C., Murry, B. A., Trant, J. M. & Mason, J. I. (1990). Human 3 beta-
hydroxysteroid dehydrogenase/delta 5----4isomerase from placenta: expression in
nonsteroidogenic cells of a protein that catalyzes the dehydrogenation/isomerization
of C21 and C19 steroids. Endocrinology 126, 2493-8.
20. Rheaume, E., Lachance, Y., Zhao, H. F., Breton, N., Dumont, M., de Launoit, Y.,
Trudel, C., Luu-The, V., Simard, J. & Labrie, F. (1991). Structure and expression of
a new complementary DNA encoding the almost exclusive 3 beta-hydroxysteroid
dehydrogenase/delta 5-delta 4-isomerase in human adrenals and gonads. Mol
Endocrinol 5, 1147-57.
140
21. Russell, D. W. & Wilson, J. D. (1994). Steroid 5 alpha-reductase: two genes/two
enzymes. Annu Rev Biochem 63, 25-61.
22. Thigpen, A. E., Silver, R. I., Guileyardo, J. M., Casey, M. L., McConnell, J. D. &
Russell, D. W. (1993). Tissue distribution and ontogeny of steroid 5 alpha-reductase
isozyme expression. J Clin Invest 92, 903-10.
23. Suzuki, T., Miki, Y., Nakamura, Y., Moriya, T., Ito, K., Ohuchi, N. & Sasano, H.
(2005). Sex steroid-producing enzymes in human breast cancer. Endocr Relat
Cancer 12, 701-20.
24. Thompson, E. A., Jr. & Siiteri, P. K. (1974). Utilization of oxygen and reduced
nicotinamide adenine dinucleotide phosphate by human placental microsomes
during aromatization of androstenedione. J Biol Chem 249, 5364-72.
25. Simpson, E. R., Mahendroo, M. S., Means, G. D., Kilgore, M. W., Hinshelwood, M.
M., Graham-Lorence, S., Amarneh, B., Ito, Y., Fisher, C. R., Michael, M. D. & et al.
(1994). Aromatase cytochrome P450, the enzyme responsible for estrogen
biosynthesis. Endocr Rev 15, 342-55.
26. Ghosh, D., Griswold, J., Erman, M. & Pangborn, W. (2009). Structural basis for
androgen specificity and oestrogen synthesis in human aromatase. Nature 457, 219-
23.
27. Penning, T. M., Burczynski, M. E., Jez, J. M., Hung, C. F., Lin, H. K., Ma, H.,
Moore, M., Palackal, N. & Ratnam, K. (2000). Human 3alpha-hydroxysteroid
dehydrogenase isoforms (AKR1C1-AKR1C4) of the aldo-keto reductase
superfamily: functional plasticity and tissue distribution reveals roles in the
inactivation and formation of male and female sex hormones. Biochem J 351, 67-77.
28. Barski, O. A., Tipparaju, S. M. & Bhatnagar, A. (2008). The aldo-keto reductase
superfamily and its role in drug metabolism and detoxification. Drug Metab Rev 40,
553-624.
29. Penning, T. M., Jin, Y., Rizner, T. L. & Bauman, D. R. (2008). Pre-receptor
regulation of the androgen receptor. Mol Cell Endocrinol 281, 1-8.
30. Henderson, B. E., Ross, R. K., Pike, M. C. & Casagrande, J. T. (1982). Endogenous
hormones as a major factor in human cancer. Cancer Res 42, 3232-9.
141
31. Dunn, B. K. & Ford, L. G. (2007). Hormonal interventions to prevent hormonal
cancers: breast and prostate cancers. Eur J Cancer Prev 16, 232-42.
32. Henderson, B. E. & Feigelson, H. S. (2000). Hormonal carcinogenesis.
Carcinogenesis 21, 427-33.
33. Clemons, M. & Goss, P. (2001). Estrogen and the risk of breast cancer. N Engl J
Med 344, 276-85.
34. Yager, J. D. & Davidson, N. E. (2006). Estrogen carcinogenesis in breast cancer. N
Engl J Med 354, 270-82.
35. Cavalieri, E., Frenkel, K., Liehr, J. G., Rogan, E. & Roy, D. (2000). Estrogens as
endogenous genotoxic agents--DNA adducts and mutations. J Natl Cancer Inst
Monogr, 75-93.
36. Dunn, B. K., Wickerham, D. L. & Ford, L. G. (2005). Prevention of hormone-
related cancers: breast cancer. J Clin Oncol 23, 357-67.
37. Miller, W. R. (1991). Aromatase activity in breast tissue. J Steroid Biochem Mol
Biol 39, 783-90.
38. Siegelmann-Danieli, N. & Buetow, K. H. (1999). Constitutional genetic variation at
the human aromatase gene (Cyp19) and breast cancer risk. Br J Cancer 79, 456-63.
39. Ross, R. K., Pike, M. C., Coetzee, G. A., Reichardt, J. K., Yu, M. C., Feigelson, H.,
Stanczyk, F. Z., Kolonel, L. N. & Henderson, B. E. (1998). Androgen metabolism
and prostate cancer: establishing a model of genetic susceptibility. Cancer Res 58,
4497-504.
40. Huggins, C. & Hodges, C. V. (1941). Studies on prostatic cancer - I The effect of
castration, of estrogen and of androgen injection on serum phosphatases in
metastatic carcinoma of the prostate. Cancer Res 1, 293-7.
41. Hsing, A. W., Reichardt, J. K. & Stanczyk, F. Z. (2002). Hormones and prostate
cancer: current perspectives and future directions. Prostate 52, 213-35.
42. Makridakis, N. M. & Reichardt, J. K. (2001). Molecular epidemiology of hormone-
metabolic loci in prostate cancer. Epidemiol Rev 23, 24-9.
43. McPhaul, M. J. (1999). Molecular defects of the androgen receptor. J Steroid
Biochem Mol Biol 69, 315-22.
142
44. Sharifi, N. & Auchus, R. J. (2012). Steroid biosynthesis and prostate cancer.
Steroids 77, 719-26.
45. Jaffe, J. M., Malkowicz, S. B., Walker, A. H., MacBride, S., Peschel, R.,
Tomaszewski, J., Van Arsdalen, K., Wein, A. J. & Rebbeck, T. R. (2000).
Association of SRD5A2 genotype and pathological characteristics of prostate
tumors. Cancer Res 60, 1626-30.
46. Deyashiki, Y., Ogasawara, A., Nakayama, T., Nakanishi, M., Miyabe, Y., Sato, K.
& Hara, A. (1994). Molecular cloning of two human liver 3 alpha-
hydroxysteroid/dihydrodiol dehydrogenase isoenzymes that are identical with
chlordecone reductase and bile-acid binder. Biochem J 299 (Pt 2), 545-52.
47. Jez, J. M., Flynn, T. G. & Penning, T. M. (1997). A new nomenclature for the aldo-
keto reductase superfamily. Biochem Pharmacol 54, 639-47.
48. Penning, T. M., Jin, Y., Steckelbroeck, S., Lanisnik Rizner, T. & Lewis, M. (2004).
Structure-function of human 3 alpha-hydroxysteroid dehydrogenases: genes and
proteins. Mol Cell Endocrinol 215, 63-72.
49. Khanna, M., Qin, K. N., Wang, R. W. & Cheng, K. C. (1995). Substrate specificity,
gene structure, and tissue-specific distribution of multiple human 3 alpha-
hydroxysteroid dehydrogenases. J Biol Chem 270, 20162-8.
50. Dufort, I., Labrie, F. & Luu-The, V. (2001). Human types 1 and 3 3 alpha-
hydroxysteroid dehydrogenases: differential lability and tissue distribution. J Clin
Endocrinol Metab 86, 841-6.
51. Bennett, M. J., Albert, R. H., Jez, J. M., Ma, H., Penning, T. M. & Lewis, M. (1997).
Steroid recognition and regulation of hormone action: crystal structure of
testosterone and NADP+ bound to 3 alpha-hydroxysteroid/dihydrodiol
dehydrogenase. Structure 5, 799-812.
52. Nahoum, V., Gangloff, A., Legrand, P., Zhu, D. W., Cantin, L., Zhorov, B. S., Luu-
The, V., Labrie, F., Breton, R. & Lin, S. X. (2001). Structure of the human 3alpha-
hydroxysteroid dehydrogenase type 3 in complex with testosterone and NADP at
1.25-A resolution. J Biol Chem 276, 42091-8.
53. Jin, Y., Stayrook, S. E., Albert, R. H., Palackal, N. T., Penning, T. M. & Lewis, M.
(2001). Crystal structure of human type III 3alpha-hydroxysteroid
143
dehydrogenase/bile acid binding protein complexed with NADP(+) and
ursodeoxycholate. Biochemistry 40, 10161-8.
54. Couture, J. F., Legrand, P., Cantin, L., Luu-The, V., Labrie, F. & Breton, R. (2003).
Human 20alpha-hydroxysteroid dehydrogenase: crystallographic and site-directed
mutagenesis studies lead to the identification of an alternative binding site for C21-
steroids. J Mol Biol 331, 593-604.
55. Pollak, N., Dolle, C. & Ziegler, M. (2007). The power to reduce: pyridine
nucleotides--small molecules with a multitude of functions. Biochem J 402, 205-18.
56. Deyashiki, Y., Tamada, Y., Miyabe, Y., Nakanishi, M., Matsuura, K. & Hara, A.
(1995). Expression and kinetic properties of a recombinant 3 alpha-
hydroxysteroid/dihydrodiol dehydrogenase isoenzyme of human liver. J Biochem
118, 285-90.
57. Winters, C. J., Molowa, D. T. & Guzelian, P. S. (1990). Isolation and
characterization of cloned cDNAs encoding human liver chlordecone reductase.
Biochemistry 29, 1080-7.
58. Steckelbroeck, S., Jin, Y., Gopishetty, S., Oyesanmi, B. & Penning, T. M. (2004).
Human cytosolic 3alpha-hydroxysteroid dehydrogenases of the aldo-keto reductase
superfamily display significant 3beta-hydroxysteroid dehydrogenase activity:
implications for steroid hormone metabolism and action. J Biol Chem 279, 10784-
95.
59. Dufort, I., Rheault, P., Huang, X. F., Soucy, P. & Luu-The, V. (1999).
Characteristics of a highly labile human type 5 17beta-hydroxysteroid
dehydrogenase. Endocrinology 140, 568-74.
60. El-Alfy, M., Luu-The, V., Huang, X. F., Berger, L., Labrie, F. & Pelletier, G.
(1999). Localization of type 5 17beta-hydroxysteroid dehydrogenase, 3beta-
hydroxysteroid dehydrogenase, and androgen receptor in the human prostate by in
situ hybridization and immunocytochemistry. Endocrinology 140, 1481-91.
61. Luu-The, V., Dufort, I., Pelletier, G. & Labrie, F. (2001). Type 5 17beta-
hydroxysteroid dehydrogenase: its role in the formation of androgens in women.
Mol Cell Endocrinol 171, 77-82.
144
62. Oduwole, O. O., Li, Y., Isomaa, V. V., Mantyniemi, A., Pulkka, A. E., Soini, Y. &
Vihko, P. T. (2004). 17beta-hydroxysteroid dehydrogenase type 1 is an independent
prognostic marker in breast cancer. Cancer Res 64, 7604-9.
63. Vihko, P., Herrala, A., Harkonen, P., Isomaa, V., Kaija, H., Kurkela, R., Li, Y.,
Patrikainen, L., Pulkka, A., Soronen, P. & Torn, S. (2005). Enzymes as modulators
in malignant transformation. J Steroid Biochem Mol Biol 93, 277-83.
64. Qiu, W., Zhou, M., Labrie, F. & Lin, S. X. (2004). Crystal structures of the
multispecific 17beta-hydroxysteroid dehydrogenase type 5: critical androgen
regulation in human peripheral tissues. Mol Endocrinol 18, 1798-807.
65. Komoto, J., Yamada, T., Watanabe, K. & Takusagawa, F. (2004). Crystal structure
of human prostaglandin F synthase (AKR1C3). Biochemistry 43, 2188-98.
66. Lovering, A. L., Ride, J. P., Bunce, C. M., Desmond, J. C., Cummings, S. M. &
White, S. A. (2004). Crystal structures of prostaglandin D(2) 11-ketoreductase
(AKR1C3) in complex with the nonsteroidal anti-inflammatory drugs flufenamic
acid and indomethacin. Cancer Res 64, 1802-10.
67. Qiu, W., Zhou, M., Mazumdar, M., Azzi, A., Ghanmi, D., Luu-The, V., Labrie, F.
& Lin, S. X. (2007). Structure-based inhibitor design for an enzyme that binds
different steroids: a potent inhibitor for human type 5 17beta-hydroxysteroid
dehydrogenase. J Biol Chem 282, 8368-79.
68. Zhang, Y., Dufort, I., Rheault, P. & Luu-The, V. (2000). Characterization of a
human 20alpha-hydroxysteroid dehydrogenase. J Mol Endocrinol 25, 221-8.
69. Nishizawa, M., Nakajima, T., Yasuda, K., Kanzaki, H., Sasaguri, Y., Watanabe, K.
& Ito, S. (2000). Close kinship of human 20alpha-hydroxysteroid dehydrogenase
gene with three aldo-keto reductase genes. Genes Cells 5, 111-25.
70. Piekorz, R. P., Gingras, S., Hoffmeyer, A., Ihle, J. N. & Weinstein, Y. (2005).
Regulation of progesterone levels during pregnancy and parturition by signal
transducer and activator of transcription 5 and 20alpha-hydroxysteroid
dehydrogenase. Mol Endocrinol 19, 431-40.
71. Higaki, Y., Usami, N., Shintani, S., Ishikura, S., El-Kabbani, O. & Hara, A. (2003).
Selective and potent inhibitors of human 20alpha-hydroxysteroid dehydrogenase
145
(AKR1C1) that metabolizes neurosteroids derived from progesterone. Chem Biol
Interact 143-144, 503-13.
72. Ji, Q., Aoyama, C., Nien, Y. D., Liu, P. I., Chen, P. K., Chang, L., Stanczyk, F. Z.
& Stolz, A. (2004). Selective loss of AKR1C1 and AKR1C2 in breast cancer and
their potential effect on progesterone signaling. Cancer Res 64, 7610-7.
73. Dufort, I., Soucy, P., Labrie, F. & Luu-The, V. (1996). Molecular cloning of human
type 3 3 alpha-hydroxysteroid dehydrogenase that differs from 20 alpha-
hydroxysteroid dehydrogenase by seven amino acids. Biochem Biophys Res
Commun 228, 474-9.
74. Matsuura, K., Deyashiki, Y., Sato, K., Ishida, N., Miwa, G. & Hara, A. (1997).
Identification of amino acid residues responsible for differences in substrate
specificity and inhibitor sensitivity between two human liver dihydrodiol
dehydrogenase isoenzymes by site-directed mutagenesis. Biochem J 323 (Pt 1), 61-
4.
75. Rizner, T. L., Lin, H. K., Peehl, D. M., Steckelbroeck, S., Bauman, D. R. & Penning,
T. M. (2003). Human type 3 3alpha-hydroxysteroid dehydrogenase (aldo-keto
reductase 1C2) and androgen metabolism in prostate cells. Endocrinology 144,
2922-32.
76. Ji, Q., Chang, L., VanDenBerg, D., Stanczyk, F. Z. & Stolz, A. (2003). Selective
reduction of AKR1C2 in prostate cancer and its role in DHT metabolism. Prostate
54, 275-89.
77. Siiteri, P. K. & Wilson, J. D. (1970). Dihydrotestosterone in prostatic hypertrophy. I.
The formation and content of dihydrotestosterone in the hypertrophic prostate of
man. J Clin Invest 49, 1737-45.
78. Ji, Q., Chang, L., Stanczyk, F. Z., Ookhtens, M., Sherrod, A. & Stolz, A. (2007).
Impaired dihydrotestosterone catabolism in human prostate cancer: critical role of
AKR1C2 as a pre-receptor regulator of androgen receptor signaling. Cancer Res 67,
1361-9.
79. Huang, K. H., Chiou, S. H., Chow, K. C., Lin, T. Y., Chang, H. W., Chiang, I. P. &
Lee, M. C. (2010). Overexpression of aldo-keto reductase 1C2 is associated with
disease progression in patients with prostatic cancer. Histopathology 57, 384-94.
146
80. Lewis, M. J., Wiebe, J. P. & Heathcote, J. G. (2004). Expression of progesterone
metabolizing enzyme genes (AKR1C1, AKR1C2, AKR1C3, SRD5A1, SRD5A2) is
altered in human breast carcinoma. BMC Cancer 4, 27.
81. Stolz, A., Hammond, L., Lou, H., Takikawa, H., Ronk, M. & Shively, J. E. (1993).
cDNA cloning and expression of the human hepatic bile acid-binding protein. A
member of the monomeric reductase gene family. J Biol Chem 268, 10448-57.
82. Hara, A., Matsuura, K., Tamada, Y., Sato, K., Miyabe, Y., Deyashiki, Y. & Ishida,
N. (1996). Relationship of human liver dihydrodiol dehydrogenases to hepatic bile-
acid-binding protein and an oxidoreductase of human colon cells. Biochem J 313
(Pt 2), 373-6.
83. Griffin, L. D. & Mellon, S. H. (1999). Selective serotonin reuptake inhibitors
directly alter activity of neurosteroidogenic enzymes. Proc Natl Acad Sci U S A 96,
13512-7.
84. Veilleux, A., Cote, J. A., Blouin, K., Nadeau, M., Pelletier, M., Marceau, P.,
Laberge, P. Y., Luu-The, V. & Tchernof, A. (2012). Glucocorticoid-induced
androgen inactivation by aldo-keto reductase 1C2 promotes adipogenesis in human
preadipocytes. Am J Physiol Endocrinol Metab 302, E941-9.
85. Steiner, A. Z., Chang, L., Ji, Q., Ookhtens, M., Stolz, A., Paulson, R. J. & Stanczyk,
F. Z. (2008). 3alpha-Hydroxysteroid dehydrogenase type III deficiency: a novel
mechanism for hirsutism. J Clin Endocrinol Metab 93, 1298-303.
86. Couture, J. F., de Jesus-Tran, K. P., Roy, A. M., Cantin, L., Cote, P. L., Legrand, P.,
Luu-The, V., Labrie, F. & Breton, R. (2005). Comparison of crystal structures of
human type 3 3alpha-hydroxysteroid dehydrogenase reveals an "induced-fit"
mechanism and a conserved basic motif involved in the binding of androgen.
Protein Sci 14, 1485-97.
87. Wilson, D. K., Bohren, K. M., Gabbay, K. H. & Quiocho, F. A. (1992). An unlikely
sugar substrate site in the 1.65 A structure of the human aldose reductase
holoenzyme implicated in diabetic complications. Science 257, 81-4.
88. Borhani, D. W., Harter, T. M. & Petrash, J. M. (1992). The crystal structure of the
aldose reductase.NADPH binary complex. J Biol Chem 267, 24841-7.
147
89. Penning, T. M. (1999). Molecular determinants of steroid recognition and catalysis
in aldo-keto reductases. Lessons from 3alpha-hydroxysteroid dehydrogenase. J
Steroid Biochem Mol Biol 69, 211-25.
90. Hoog, S. S., Pawlowski, J. E., Alzari, P. M., Penning, T. M. & Lewis, M. (1994).
Three-dimensional structure of rat liver 3 alpha-hydroxysteroid/dihydrodiol
dehydrogenase: a member of the aldo-keto reductase superfamily. Proc Natl Acad
Sci U S A 91, 2517-21.
91. Schlegel, B. P., Jez, J. M. & Penning, T. M. (1998). Mutagenesis of 3 alpha-
hydroxysteroid dehydrogenase reveals a "push-pull" mechanism for proton transfer
in aldo-keto reductases. Biochemistry 37, 3538-48.
92. Jin, Y. & Penning, T. M. (2006). Multiple steps determine the overall rate of the
reduction of 5alpha-dihydrotestosterone catalyzed by human type 3 3alpha-
hydroxysteroid dehydrogenase: implications for the elimination of androgens.
Biochemistry 45, 13054-63.
93. Olefsky, J. M. (2001). Nuclear receptor minireview series. J Biol Chem 276, 36863-
4.
94. Huang, P., Chandra, V. & Rastinejad, F. (2010). Structural overview of the nuclear
receptor superfamily: insights into physiology and therapeutics. Annu Rev Physiol
72, 247-72.
95. Gronemeyer, H., Gustafsson, J. A. & Laudet, V. (2004). Principles for modulation
of the nuclear receptor superfamily. Nat Rev Drug Discov 3, 950-64.
96. Nagy, L. & Schwabe, J. W. (2004). Mechanism of the nuclear receptor molecular
switch. Trends Biochem Sci 29, 317-24.
97. Overington, J. P., Al-Lazikani, B. & Hopkins, A. L. (2006). How many drug targets
are there? Nat Rev Drug Discov 5, 993-6.
98. Heldring, N., Pike, A., Andersson, S., Matthews, J., Cheng, G., Hartman, J.,
Tujague, M., Strom, A., Treuter, E., Warner, M. & Gustafsson, J. A. (2007).
Estrogen receptors: how do they signal and what are their targets. Physiol Rev 87,
905-31.
148
99. Walter, P., Green, S., Greene, G., Krust, A., Bornert, J. M., Jeltsch, J. M., Staub, A.,
Jensen, E., Scrace, G., Waterfield, M. & et al. (1985). Cloning of the human
estrogen receptor cDNA. Proc Natl Acad Sci U S A 82, 7889-93.
100. Greene, G. L., Gilna, P., Waterfield, M., Baker, A., Hort, Y. & Shine, J. (1986).
Sequence and expression of human estrogen receptor complementary DNA. Science
231, 1150-4.
101. Kuiper, G. G., Enmark, E., Pelto-Huikko, M., Nilsson, S. & Gustafsson, J. A.
(1996). Cloning of a novel receptor expressed in rat prostate and ovary. Proc Natl
Acad Sci U S A 93, 5925-30.
102. Ogawa, S., Inoue, S., Watanabe, T., Hiroi, H., Orimo, A., Hosoi, T., Ouchi, Y. &
Muramatsu, M. (1998). The complete primary structure of human estrogen receptor
beta (hER beta) and its heterodimerization with ER alpha in vivo and in vitro.
Biochem Biophys Res Commun 243, 122-6.
103. Ascenzi, P., Bocedi, A. & Marino, M. (2006). Structure-function relationship of
estrogen receptor alpha and beta: impact on human health. Mol Aspects Med 27,
299-402.
104. Gustafsson, J. A. (2003). What pharmacologists can learn from recent advances in
estrogen signalling. Trends Pharmacol Sci 24, 479-85.
105. Lavery, D. N. & McEwan, I. J. (2005). Structure and function of steroid receptor
AF1 transactivation domains: induction of active conformations. Biochem J 391,
449-64.
106. McEwan, I. J. & Nardulli, A. M. (2009). Nuclear hormone receptor architecture -
form and dynamics: The 2009 FASEB Summer Conference on Dynamic Structure
of the Nuclear Hormone Receptors. Nucl Recept Signal 7, e011.
107. Chouard, T. (2011). Structural biology: Breaking the protein rules. Nature 471, 151-
3.
108. Schwabe, J. W., Neuhaus, D. & Rhodes, D. (1990). Solution structure of the DNA-
binding domain of the oestrogen receptor. Nature 348, 458-61.
109. Schwabe, J. W., Chapman, L., Finch, J. T. & Rhodes, D. (1993). The crystal
structure of the estrogen receptor DNA-binding domain bound to DNA: how
receptors discriminate between their response elements. Cell 75, 567-78.
149
110. Schwabe, J. W., Chapman, L., Finch, J. T., Rhodes, D. & Neuhaus, D. (1993). DNA
recognition by the oestrogen receptor: from solution to the crystal. Structure 1, 187-
204.
111. Brzozowski, A. M., Pike, A. C., Dauter, Z., Hubbard, R. E., Bonn, T., Engstrom, O.,
Ohman, L., Greene, G. L., Gustafsson, J. A. & Carlquist, M. (1997). Molecular
basis of agonism and antagonism in the oestrogen receptor. Nature 389, 753-8.
112. Tanenbaum, D. M., Wang, Y., Williams, S. P. & Sigler, P. B. (1998).
Crystallographic comparison of the estrogen and progesterone receptor's ligand
binding domains. Proc Natl Acad Sci U S A 95, 5998-6003.
113. Shiau, A. K., Barstad, D., Loria, P. M., Cheng, L., Kushner, P. J., Agard, D. A. &
Greene, G. L. (1998). The structural basis of estrogen receptor/coactivator
recognition and the antagonism of this interaction by tamoxifen. Cell 95, 927-37.
114. Skafar, D. F. & Zhao, C. (2008). The multifunctional estrogen receptor-alpha F
domain. Endocrine 33, 1-8.
115. Pratt, W. B. & Toft, D. O. (2003). Regulation of signaling protein function and
trafficking by the hsp90/hsp70-based chaperone machinery. Exp Biol Med
(Maywood) 228, 111-33.
116. Cheung, E. & Kraus, W. L. (2010). Genomic analyses of hormone signaling and
gene regulation. Annu Rev Physiol 72, 191-218.
117. Ellmann, S., Sticht, H., Thiel, F., Beckmann, M. W., Strick, R. & Strissel, P. L.
(2009). Estrogen and progesterone receptors: from molecular structures to clinical
targets. Cell Mol Life Sci 66, 2405-26.
118. Pearce, S. T. & Jordan, V. C. (2004). The biological role of estrogen receptors alpha
and beta in cancer. Crit Rev Oncol Hematol 50, 3-22.
119. Alland, L., Muhle, R., Hou, H., Jr., Potes, J., Chin, L., Schreiber-Agus, N. &
DePinho, R. A. (1997). Role for N-CoR and histone deacetylase in Sin3-mediated
transcriptional repression. Nature 387, 49-55.
120. Nagy, L., Kao, H. Y., Chakravarti, D., Lin, R. J., Hassig, C. A., Ayer, D. E.,
Schreiber, S. L. & Evans, R. M. (1997). Nuclear receptor repression mediated by a
complex containing SMRT, mSin3A, and histone deacetylase. Cell 89, 373-80.
150
121. Bain, D. L., Heneghan, A. F., Connaghan-Jones, K. D. & Miura, M. T. (2007).
Nuclear receptor structure: implications for function. Annu Rev Physiol 69, 201-20.
122. Jordan, V. C. (2001). Selective estrogen receptor modulation: a personal perspective.
Cancer Res 61, 5683-7.
123. Shang, Y. & Brown, M. (2002). Molecular determinants for the tissue specificity of
SERMs. Science 295, 2465-8.
124. Luisi, B. F., Xu, W. X., Otwinowski, Z., Freedman, L. P., Yamamoto, K. R. &
Sigler, P. B. (1991). Crystallographic analysis of the interaction of the
glucocorticoid receptor with DNA. Nature 352, 497-505.
125. Chen, Y. & Young, M. A. (2010). Structure of a thyroid hormone receptor DNA-
binding domain homodimer bound to an inverted palindrome DNA response
element. Mol Endocrinol 24, 1650-64.
126. Gewirth, D. T. & Sigler, P. B. (1995). The basis for half-site specificity explored
through a non-cognate steroid receptor-DNA complex. Nat Struct Biol 2, 386-94.
127. Rastinejad, F., Perlmann, T., Evans, R. M. & Sigler, P. B. (1995). Structural
determinants of nuclear receptor assembly on DNA direct repeats. Nature 375, 203-
11.
128. Williams, S. P. & Sigler, P. B. (1998). Atomic structure of progesterone complexed
with its receptor. Nature 393, 392-6.
129. Zhao, Q., Chasse, S. A., Devarakonda, S., Sierk, M. L., Ahvazi, B. & Rastinejad, F.
(2000). Structural basis of RXR-DNA interactions. J Mol Biol 296, 509-20.
130. Meijsing, S. H., Pufall, M. A., So, A. Y., Bates, D. L., Chen, L. & Yamamoto, K. R.
(2009). DNA binding site sequence directs glucocorticoid receptor structure and
activity. Science 324, 407-10.
131. Chandra, V., Huang, P., Hamuro, Y., Raghuram, S., Wang, Y., Burris, T. P. &
Rastinejad, F. (2008). Structure of the intact PPAR-gamma-RXR-alpha nuclear
receptor complex on DNA. Nature 456, 350-356.
132. Figueira, A. C., Lima, L. M., Lima, L. H., Ranzani, A. T., Mule Gdos, S. &
Polikarpov, I. (2010). Recognition by the thyroid hormone receptor of canonical
DNA response elements. Biochemistry 49, 893-904.
151
133. Zhang, J., Chalmers, M. J., Stayrook, K. R., Burris, L. L., Wang, Y., Busby, S. A.,
Pascal, B. D., Garcia-Ordonez, R. D., Bruning, J. B., Istrate, M. A., Kojetin, D. J.,
Dodge, J. A., Burris, T. P. & Griffin, P. R. (2011). DNA binding alters coactivator
interaction surfaces of the intact VDR-RXR complex. Nat Struct Mol Biol 18, 556-
63.
134. Surjit, M., Ganti, K. P., Mukherji, A., Ye, T., Hua, G., Metzger, D., Li, M. &
Chambon, P. (2011). Widespread negative response elements mediate direct
repression by agonist-liganded glucocorticoid receptor. Cell 145, 224-41.
152