sulfur-36s stable isotope labeling of amino acids for quantification (sulaq)
TRANSCRIPT
TECHNICAL BRIEF
Sulfur-36S stable isotope labeling of amino acids
for quantification (SULAQ)
Nico Jehmlich1,5, Frank-Dieter Kopinke2, Steffi Lenhard1,3, Carsten Vogt4, Florian-AlexanderHerbst1, Jana Seifert1, Ulrike Lissner 5, Uwe Volker 5, Frank Schmidt1,5 and Martin von Bergen1,6
1 Department of Proteomics, Helmholtz Centre for Environmental Research – UFZ, Leipzig, Germany2 Department of Environmental Engineering, Helmholtz Centre for Environmental Research – UFZ, Leipzig,
Germany3 Biotechnology Center of the TU Dresden, Tatzberg, Dresden, Germany4 Department of Isotope Biogeochemistry, Helmholtz Centre for Environmental Research – UFZ, Leipzig, Germany5 Department of Functional Genomics, Interfaculty Institute for Genetics and Functional Genomics, Ernst-Moritz-
Arndt-University, Greifswald, Germany6 Department of Metabolomics, Helmholtz Centre for Environmental Research – UFZ, Leipzig, Germany
Received: February 1, 2011
Revised: October 12, 2011
Accepted: October 25, 2011
We introduce a universal metabolic labeling strategy using elemental heavy 36Sulfur (36S)
called 36Sulfur stable isotope labeling of amino acids for quantification (SULAQ). In the proof
of principle experiment, Pseudomonas putida KT2440 was grown in defined minimal medium
with sodium benzoate or sodium succinate as the sole carbon and 32S- or 36S-sodium sulfate
as the sole sulfur sources. Quantification using mass spectrometry resulted in 562 proteins
with 1991 unique peptides. SULAQ technology can be a valuable alternative strategy for the
quantitative comparisons in MS-based proteomics approaches characterizing bacterial and
other biological samples in different growth conditions.
Keywords:
Cysteine / Metabolic labeling / Methionine / Pseudomonas putida / Stable isotope
labeling / 36Sulfur incorporation / Technology
Mass spectrometry (MS) is the method of choice in
proteomics for protein identification due to remarkable
improvements in mass accuracy, sensitivity and speed.
Besides protein identification, relative quantification of
dynamic changes in the proteome plays a key role in nearly
all systems biology approaches.
In the past two decades, several quantitative proteomics
techniques coupling stable isotope labeling and MS-analysis
have been successfully developed. In these studies, two
or more biological samples are cultivated under
two different conditions: one sample is cultivated in
light media and one sample in medium with heavy
isotopes. By means of high mass accuracy MS, isotope
clusters of each stable isotope can be measured and the
intensities of light and heavy peptides can be used to
calculate the relative amount of proteins. Up to now,
stable hydrogen, carbon or nitrogen isotopes (2H, 13C, or15N) have been provided as inorganic salts or labeled
organic carbon sources as well as amino acids have been
used to label newly synthesized proteins (for review
see [1, 2]). Besides these dominating elements of the
protein backbone, the chemical element sulfur (S) is also
ubiquitous in all natural proteomes, because it is incorpo-
rated into the side chains of cysteine and methionine, and
plays a central role in cell metabolism, cell physiology and
health [3]. An overview of absolute quantitation of thiol
and sulfur-containing amino acid metabolites in yeast
extracts by MS-based methods is decribed (see review [4]).Abbreviation: SULAQ, 36S stable isotope labeling for MS-based
quantification
Correspondence: Dr. Frank Schmidt, Interfaculty Institute for
Genetics and Functional Genomics, Department of Functional
Genomics, Ernst-Moritz-Arndt-University Greifswald, Friedrich-
Ludwig-Jahn-Strasse 15a, 17487 Greifswald, Germany
E-mail: [email protected]
Fax: 149-3834-86-795871
& 2011 WILEY-VCH Verlag GmbH & Co. KGaA, Weinheim www.proteomics-journal.com
Proteomics 2012, 12, 37–42 37DOI 10.1002/pmic.201100057
For metabolic labeling of proteins, stable isotope labeling
by amino acids in cell culture (SILAC) using 15N- and 13C-
containing amino acids is the ‘gold standard’ [5]. SILAC has
been applied in numerous quantitative proteomics analyses,
demonstrating its potential as a powerful and versatile
approach for proteome-wide quantification, which can also
be extended to the monitoring of post-translational modifi-
cations, e.g. protein phosphorylation [6–9]. The strength of
the SILAC approach is based on the predictable incorpora-
tion of amino acids resulting into well-defined mass shifts.
A B FractionationCultivation
Pseudomonas putida KT2440
control
SDS-PAGE1200
kDa
stress condition
85100120150
Sulfurminimalmedium
506070
Na2SO4Na-benzoate
Na2SO4Na-succinate
40
Sample preparation andprotein extract mixed 1:1 N
umbe
r of
cut
ted
band
s
30
25
20
nanoLC-Orbitrap MS/MS24
15
Database search and data analysis Observation of retention time shiftC D
Δ RT min (heavy labeled non-oxidized peptidesvs. heavy labeled oxidized peptides)
Chromatogram View
Δ RT min (heavy labeled oxidized peptidesvs. light unlabeled oxidized peptides)
light - unlabeled
heavy - labeled
Δ 3.02 minSpectrum View retention time [min] peptide-
heavy - labeledlight -unlabeled- SFAFGSISSTSGSLM(heavy)PR -non-oxidized pair
peptide-SFAFGSISSTSGSLM (heavy/ox)PR -
m/zrela
tive
ab
un
dan
ce [
%]
32 36 40 44
oxidized pair
retention time [min]
E Quantitative interpretation
Control analysis Biological analysis
32S / 36S 1:1 mixture5
Benzoate / Succinategel-free, n=284 1D-PAGE, n=5625
100 200 300
0
log
2 ra
tio
200 400 600
0
log
2 ra
tio
-5number of proteins
-5number of proteins
Example: IGIMPGHIHLPGK, Charge =4, Δ =1.002 m/z
36S32S
25.2 25.8 26.4 27.0
38 N. Jehmlich et al. Proteomics 2012, 12, 37–42
& 2011 WILEY-VCH Verlag GmbH & Co. KGaA, Weinheim www.proteomics-journal.com
In contrast, methods using stable isotope labeled substrates
instead of labeled amino acids require metabolization by
microbes potentially resulting in unpredictable and dynamic
incorporation into proteins [10].
Microorganisms are very versatile in terms of their
physiological capabilities and are thus also capable of
synthesizing amino acids de novo. Owing to this fact the
application of SILAC to microbes is limited to strains
that are auxotrophic for at least one abundant amino acid
[11, 12].
In this study, we introduce an alternative metabolic
labeling strategy using heavy sulfur 36S stable isotope
labeling for MS-based quantification (SULAQ). This strategy
meets the following requirements for valuable quantifica-
tion approaches: easy distinction of sample and control,
accurate quantification, comprehensive coverage of the
proteome and high-throughput capacity. The incorporation
of 36S into defined amino acids has several advantages for
quantitative protein analysis: (i) a constant mass shift
between the control versus treated sample of 4 Da for each
sulfur-containing amino acid per peptide, (ii) incorporation
into cysteine allows the implementation of cysteine-specific
tagging strategies for enrichment [13], or direct probing by
disulfide exchange chromatography [14, 15], and (iii) enables
chromatographic isolation of either cysteine- or methionine-
containing peptides using combined fractional diagonal
chromatography (COFRADIC) [16, 17].
In the past, metabolic incorporation of radioactively
labeled amino acids such as 35S-methionine and -cysteine
was used succesfully in several applications to study
e.g. the proteome response to oxidative stress in Sacchar-omyces cerevisiae [18] or Candida albicans [19], intracellular
proteolysis patterns of Bacillus subtilis during glucose star-
vation [20], or the thiolation of the Arabidopsis thalianaproteome [21]. However, radioactive material requires
appropiate safety precautions. For example, 35S-labeled
solutions have been found to release volatile radioactive
substances [22] and are therefore not applicable in standard
laboratories.
Therefore, alternative labeling strategies are still needed
to facilitate quantitative approaches, particularly for micro-
bial proteomics in order to gain new insights into such
important fields like infection biology, biotechnology and
environmental microbiology.
In order to verify the 36S incorporation rate, time
constant and proteome stability, the model bacterium
Pseudomonas putida KT2440 (DSM number 6125) was
cultivated containing 10 mM sodium succinate but two
different sulfur sources (32S or 36S sodium sulfate). Best-fit
calculation of the 32S and 36S P. putida growth curve was
performed using the exponential growth equation of
GraphPad Prism v5.02 that describes the growth with a
constant doubling time. The 32S culture has a doubling time
of approx. 2.08 h and the 36S culture a doubling time of
1.97 h. The rate constant (k) of both cultures were 0.33 and
0.35 and were in a comparable range suggesting minor
effects triggered by the different sulfur sources (Supporting
Information Fig. 1). In a proteome analysis of the latest
time-point (t6) we were able to quantify up to 344 proteins
(Z1 peptide used for quantification) out of 713 identified
proteins (protein prophet40.95) resulting in a media ratio
(light/heavy) of 0.27. This is proportional to a labeling effi-
ciency of 73%. To get a higher labeling efficiency, we claim
that the use of an already labeled pre-culture is necessary.
Figure 1. Schematic overview of proposed workflow. P. putida KT2440 was cultivated in batch culture in defined minimal medium with
two different carbon- and energy sources, succinate and benzoate, respectively. For quantification using SULAQ the succinate grown
culture received 36S-sodium sulfate as the sulfur source and the culture growing with succinate 32S-sodium sulfate (A). Cells of both
cultures were harvested after entry into the stationary growing phase. After sample preparation and protein extraction, the protein
extracts were mixed in equal amounts (1:1) and separated by a 15-cm-long 12.5% SDS-PAGE (B). The 1-D gel was cut into 24 bands as
indicated in the figure, followed by in-gel proteolytic digestion and nano-LC separation and Orbitrap MS/MS measurement. (C) Identi-
fication and quantification of sulfur-containing peptides were performed by the software package of Rosetta Elucidator (Ceiba solutions
v3). As an example, a chromatogram and spectrum view of a quantified 36S-labeled peptide is shown. The chromatographic view (upper
panel) of the peptide (IGIMPGHIHLPGK, charge 5 4, PP_4185, succinyl-CoA synthetase, a subunit (sucD), P. putida KT2440) indicates the
extracted ion current (XIC) of the 36S-labeled (red) peptide and the 32S-unlabeled (blue) peptide at the given retention times whereas a
detailed spectrum view of the relative abundance of the peptide peaks is indicated in the lower panel. (D) Negative retention time shifts of
oxidized peptides in comparison to their non-oxidized counterparts are shown. Upper panel, Whisker-Box-Plot displays the retention time
differences of pairs of heavy 36S-labeled non-oxidized peptides and heavy 36S-labeled oxidized peptides (n 5 231). The oxidized peptides
eluted with an average of 3.8373.48 min (n 5 231) earlier than the non-oxidized peptide (median 5 3.37 min, Whisker 5% percentile 5
1.37 min, Whisker 95% percentile 5 6.55 min). The lower Whisker-Box-Plot shows the retention time difference between heavy 36S-labeled
oxidized peptides and light 32S-unlabeled oxidized peptides. Both types of peptides (light and heavy) eluted almost at the same retention
time with an average difference of 0.00570.027 min (n 5 231) (median 5 0.002 min, Whisker 5% percentile 5�0.01 min, Whisker 95%
percentile 5 0.03 min). As an example, a detailed chromatogram view of one selected quantified peptide (SFAFGSISSTSGSLMPR,
charge 5 2, PP_0824, phosphate ABC transporter, periplasmic phosphate-binding protein, P. putida KT2440) is shown in the lower part for
which the retention time between the oxidized and non-oxidized peptide pairs (light and heavy) differed by 3.02 min. This illustrates that
the obtained ratios of oxidized and non-oxidized peptides are comparable (coefficient of determination 5 0.954). (E) Quantitative
proteome analysis can be performed with e.g. histogram calculation (log2 (ratio benzoate/succinate), n 5 562, mean 5�0.14, SD 5 1.54) or
XY-plot. To validate the quantitation values, two experiments were compared (control versus biological analysis). As a result, the control
analysis (32S versus 36S analysis; one substrate) showed only slightly changes in the proteome similar to other control experiments used
for SILAC or ICAT. On the other side, biological analysis showed a remarkable higher rate of significant regulated proteins.
3
Proteomics 2012, 12, 37–42 39
& 2011 WILEY-VCH Verlag GmbH & Co. KGaA, Weinheim www.proteomics-journal.com
As expected, the median ratios found in six analyzed
time-points continuously decreased during cultivation from
4.5 (t1) to 0.27 (t6) (Supporting Information Fig. 2), due to
the replacement of 32S by 36S. At the last time point, we
finally mixed the 32S and 36S culture using a bacteria ratio of
approx. 1:1 estimated by OD600. Subsequent proteome
analysis resulted in 725 identified proteins of which 284
proteins (Z1 peptide) could be quantified using the SULAQ
approach. The median ratio (light/heavy) was 1.32
confirming the initial light/heavy labeling ratio of 0.27 in
the 36S culture only. Five up-regulated and six down-regu-
lated proteins out of 284 quantified proteins showed a fold
change greater than 2 and a p-value o0.01 that are criteria
usually applied to detect significant biological changes
within a proteome. Four of them clearly indicating reduced
labeling turnover at time point 6 in the single 36S approach.
Remaining seven proteins were quantified based on just one
peptide quantification which accounts for only 3% of the
total single peptide quantifications. Regarding these find-
ings, we assume that quantification quality by 36S is similar
to the most common quantitation approaches such as
SILAC or 2-DE and can be successfully applied to determine
relevant biological changes in the proteome when compar-
ing different physiological states.
In the second experiment, the proteome of P. putidaKT2440 during the growth with two different carbon sources
was compared. P. putida KT2440 was cultivated in batch
cultures overnight either in minimal medium supplemented
with 2 mM sodium benzoate and 2 mM 32S-sodium sulfate
or in the same medium containing 10 mM sodium succinate
as the sole carbon source and 2 mM 36S-Na2SO4 (Fig. 1A).
Cells were incubated at 301C with horizontal shaking at
125 rpm. The synthetic minimal medium without any sulfur
source contained 760 mg/L NH4Cl, 680 mg/L KH2PO4,
871 mg/L K2HPO4, 5.5 mg/L CaCl2 � 6H2O, 0.25 mg/L Na2
MoO4 � 4H2O, 20 g/L MgCl2, pH 7.0. P. putida was preculti-
vated in minimal medium in 10 mM sodium succinate as the
carbon source and 2 mM of 32S sodium sulfate. 36S-labeled
Na2SO4 was synthesized by a three-step oxidation cascade.
Briefly, a glass vial containing about 3 mg of elemental sulfur
(from Campro Scientific, 99.24% 36S-isotopic enrichment)
was transferred into a quartz tube and purged with a
continuous air flow (20 mL/min). The quartz tube was
heated with a burner such that the sulfur evaporated and
passed the hot zone where it was oxidized into SO2 in the air-
stream. The gas flow was washed with 7 mL of water
(Millipore quality) containing 0.2 mM of NaOH in order to
absorb the resulting SO2 completely. The outlet of the gas
flow was a capillary generating a flow of small gas bubbles in
the water phase. After complete purging of the quartz tube
(30 min) the pH value of the absorption solution was still
alkaline (pH 9.33). Later, 100mL of a 30% H2O2 were added
in order to oxidize sulfite to sulfate completely. The solution
was heated to about 801C until no residual H2O2 was
detectable (about 6 h, iodide-starch test). Ion chromato-
graphic analysis of the resulting solution (diluted 1:200)
revealed 1.15 g/L sulfate (11.5 mM) and no other contam-
inating anions. This concentration corresponds to a sulfate
yield of about 97%. The solution was adjusted to pH 7.4
using diluted HCl (24mmol, yielding a final chloride
concentration of about 3 mM) and for cell cultivation 2 mM
of 36S sodium sulfate was used.
For proteome analysis, crude protein extracts were
prepared as described in [23] and the extracts containing
heavy and light sulfur were pooled in a ratio of 1:1 (32S-extract
60mg136S-extract 60mg). About 120mg of protein was sepa-
rated by 1-D gel electrophoresis (Fig. 1B) and the gel lane was
cut into 24 gel bands. In-gel digestion with trypsin (Promega,
Mannheim, Germany) was performed as previously descri-
bed [23]. Tryptic peptides were measured with a nano-LTQ-
Orbitrap-MS/MS mass spectrometer [24]. LC separation was
performed using a constant flow rate of 300 nL/min, solvent
A (2% ACN, 0.1% formic acid) mixed in a 54-min gradient
with 5–100% solvent B (98% ACN, 0.1% formic acid).
Detailed chromatographic conditions were as follows:
0–5 min isocratic 5% solvent B, 5–43 min: 5–35% solvent B,
43–48 min: 35–60% solvent B, 48–50 min isocratic 60%
solvent B, 50–52 min: 60–100% solvent B, 52–54 min isocratic
100% solvent B, reconstitution of the column with solvent A
from 54 to 64 min.
Data analysis was done using the software Rosetta
Elucidator (Ceiba Solutions v3.3.0.SP3.19, MA, USA) with the
following settings: 1000 count intensity threshold, 10 ppm
mass accuracy, 10 min alignment search distance applied
for the binning process. For quantitative analysis, the data
pairs were built using a binning tolerance of 5 ppm, a
retention time location tolerance of 0.2 min and a mass label
shift of 3.995 Da. For peptide identification the following
data-dependent settings were applied: full tryptic digest,
10 ppm precursor tolerance, 1.00 Da fragment ion mass
tolerance, mass shift of methionine and cysteine by
3.995 Da, one missed proteolytic cleavage, oxidation on
methionine as ‘variable’ modification. All data searches were
performed with SEQUEST/Sorcerer (Sorcerer v3.5, Sage-N
Research, CA, USA) using a P. putida FASTA sequence
(downloaded from NCBI repository, 2009) and identified
peptides/proteins were accepted if they exceeded a Pepti-
deTeller score of 0.8 and a ProteinTeller score of 0.95 [25,
26]. For quantification, only labeled pairs were considered if
at least one of the isotope groups in the labeled pair was
annotated by peptide identification, reaching a labeled pair
status of ‘‘good’’ (Fig. 1C).
As a result, 1991 peptides accounting for 562 proteins
were quantified using the SULAQ approach based on
methionine-containing peptides (Supporting Information
Table 1). Many of the identified and quantified proteins
belonged to important metabolic processes such as the
tricarboxylic acid (TCA) cycle (Supporting Information
Fig. 3), the sulfur metabolism (Supporting Information
Fig. 4) or the cysteine and methionine metabolism
(Supporting Information Fig. 5). So far only methionine-
containing peptides were used for quantitation.
40 N. Jehmlich et al. Proteomics 2012, 12, 37–42
& 2011 WILEY-VCH Verlag GmbH & Co. KGaA, Weinheim www.proteomics-journal.com
We also observed a subset of 231 peptide pairs with a
methionine oxidation that results in a mass shift difference
of 116 Da between the non-oxidized and oxidized peptides
(Fig. 1D). The retention times for oxidative peptides changed
during chromatography: oxidized eluted earlier (median 5
3.37 min, n 5 231) than non-oxidized peptides. This obser-
vation can be explained by the fact that oxidation of
methionine to sulfoxide or sulfone (and cysteine to sulfenic
acid, sulfinic acid and sulfonic acid) leads to a decreased
hydrophobicity, thus reducing the peptide retention time on
a reversed phase column [27]. As expected, the retention
times of the unlabeled and the heavy labeled peptides did not
differ (median 5 0.002 min, n 5 231). Furthermore, quanti-
fication of peptide intensities yielded similar data for
oxidized and the non-oxidized peptides (coefficient
R2 5 0.954). The ratios of oxidized and non-oxidized peptides
differed by only 4.8% from the average of the ratios (n 5 231,
SD 5 14.4%) and therefore both ratios can be used for rela-
tive quantification. Overall, the ability to quantify oxidized
and non-oxidized peptides is a clear benefit for targeted
methods studying e.g. oxidative damage of proteins.
After database searching and data analysis, results of
quantitative proteome analysis can be displayed in multiple
ways, e.g. histogram calculation followed by pathway and
genome database comparisons for functional analysis [28].
In order to validate our alternative labeling strategy
(SULAQ), we cultured P. putida KT2440 with succinate as
control substrate and the monocyclic aromatic compound
benzoate as the stressor substrate. However, addition of
succinate itself caused the up-regulations of several proteins
including amino acid transporters, stress proteins or anti-
oxidants [29, 30]. We were able to confirm the up-regulation
via SULAQ of the branched-chain amino acid ABC trans-
porter (PP_1141, braC) with an average fold change of �1.9
(32S-benzoate/36S-succinate) or the adenylate kinase (amino
acid metabolism, PP_1506, adk, average fold change of
�4.5) indicating higher levels of these proteins during
growth with succinate. In the presence of benzoate as
stressor, P. putida KT2440 is expected to produce higher
levels proteins involved in degradation, prevention of
uptake, and neutralization of the acid by phosphate [31]. The
degradation of benzoate is known to proceed via catechol
and the X-ketoadipate pathway [32]. Strongly increased levels
of X-ketodipyl CoA thiolase (PP_1377, pcaF, average fold
change4100) [29] were observed in our experiment in the
presence of benzoate. Increased cellular levels of succinyl-
CoA synthetase (PP_4185, sucD, average fold change 5.8)
[31] or translation elongation factor Tu (PP_0440, tuf-1,
average fold change 4.1; PP_0452, tuf-2, average fold change
3.7) are also compatible with the better growth of P. putidaKT2440 observed with benzoate.
Since the usage of sulfur-isotope-labeled substrates are
important for proteomics studies, 34S labeled substrates can
be a perfect alternative to 36S because of their favorable price
and availability. However, currently the major bottleneck for
using 34S-labeled substrates instead of 36S is that bioinfor-
matic tools for automatic cluster de-isotoping are missing
because 34S provides only a mass shift between light and
heavy isotope of 2 Da; nevertheless we believe such tool
will be available in the near future. To demonstrate a
general feasibility, we performed an additional experi-
ment using 34S instead of 36S. Initial results are promis-
ing and indicate high coverage of quantifiable peptides
and concomitantly no significantly proteome changes
using 34S (data not shown).
Our proof of principle study indicates that SULAQ is a
valuable tool for studying protein changes in microorgan-
isms. Furthermore, this labeling approach can also be
applied for the analysis of protein–protein interactions,
protein functions or signaling processes. In contrast to the
traditional proteomic set-ups, SULAQ can be also used for
detecting the sulfur flux in environmental microbiology
where sulfur-containing metabolites are metabolized.
This work was supported by funding from the BMBF withinthe framework of 01 ZIK-FunGene. Patent information: FrankSchmidt, Frank-Dieter Kopinke, and Martin von Bergen (2009).Verfahren zur relativen Quantifizierung von Peptiden nachEinbau von 36S nach metabolischer Markierung. German Patentno. DE 10 2008 043 241.
The authors have declared no conflict of interest.
References
[1] Brun, V., Masselon, C., Garin, J., Dupuis, A., Isotope dilution
strategies for absolute quantitative proteomics. J. Proteo-
mics 2009, 72, 740–749.
[2] Wilm, M., Quantitative proteomics in biological research.
Proteomics 2009, 9, 4590–4605.
[3] Claiborne, A., Yeh, J. I., Mallett, T. C., Luba, J. et al., Protein-
sulfenic acids: diverse roles for an unlikely player in enzyme
catalysis and redox regulation. Biochemistry 1999, 38,
15407–15416.
[4] Godat, E., Madalinski, G., Muller, L., Heilier, J. F. et al., Mass
spectrometry-based methods for the determination of
sulfur and related metabolite concentrations in cell extracts.
Methods Enzymol. 2010, 473, 41–76.
[5] Ong, S. E., Blagoev, B., Kratchmarova, I., Kristensen, D. B.
et al., Stable isotope labeling by amino acids in cell culture,
SILAC, as a simple and accurate approach to expression
proteomics. Mol. Cell. Proteomics 2002, 1, 376–386.
[6] Schmidt, F., Hustoft, H. K., Strozynski, M., Dimmler, C. et al.,
Quantitative proteome analysis of cisplatin-induced apop-
totic Jurkat T cells by stable isotope labeling with amino
acids in cell culture, SDS-PAGE, and LC-MALDI-TOF/TOF
MS. Electrophoresis 2007, 28, 4359–4368.
[7] Macek, B., Gnad, F., Soufi, B., Kumar, C. et al., Phospho-
proteome analysis of E. coli reveals evolutionary conser-
vation of bacterial Ser/Thr/Tyr phosphorylation. Mol. Cell.
Proteomics 2008, 7, 299–307.
Proteomics 2012, 12, 37–42 41
& 2011 WILEY-VCH Verlag GmbH & Co. KGaA, Weinheim www.proteomics-journal.com
[8] Gruhler, A., Olsen, J. V., Mohammed, S., Mortensen, P.
et al., Quantitative phosphoproteomics applied to the yeast
pheromone signaling pathway. Mol. Cell. Proteomics 2005,
4, 310–327.
[9] Ge, F., Xiao, C. L., Bi, L. J., Tao, S. C. et al., Quantitative
phosphoproteomics of proteasome inhibition in multiple
myeloma cells. PLoS One 2010, 5, e13095.
[10] Jehmlich, N., Fetzer, I., Seifert, J., Mattow, J. et al., Decimal
place slope, a fast and precise method for quantifying 13C
incorporation levels for detecting the metabolic activity of
microbial species. Mol. Cell. Proteomics 2010, 9, 1221–1227.
[11] Soufi, B., Kumar, C., Gnad, F., Mann, M. et al., Stable
isotope labeling by amino acids in cell culture (SILAC)
applied to quantitative proteomics of Bacillus subtilis.
J. Proteome Res. 2010, 9, 3638–3646.
[12] Dreisbach, A., Otto, A., Becher, D., Hammer, E. et al.,
Monitoring of changes in the membrane proteome during
stationary phase adaptation of Bacillus subtilis using in vivo
labeling techniques. Proteomics 2008, 8, 2062–2076.
[13] Schmidt, F., Dahlmann, B., Janek, K., Kloss, A. et al., Compre-
hensive quantitative proteome analysis of 20S proteasome
subtypes from rat liver by isotope coded affinity tag and 2-D
gel-based approaches. Proteomics 2006, 6, 4622–4632.
[14] Wang, S., Zhang, X., Regnier, F. E., Quantitative proteomics
strategy involving the selection of peptides containing both
cysteine and histidine from tryptic digests of cell lysates.
J. Chromatogr. A 2002, 949, 153–162.
[15] Liu, T., Qian, W. J., Chen, W. N., Jacobs, J. M. et al.,
Improved proteome coverage by using high efficiency
cysteinyl peptide enrichment: the human mammary
epithelial cell proteome. Proteomics 2005, 5, 1263–1273.
[16] Staes, A., Van Damme, P., Helsens, K., Demol, H. et al.,
Improved recovery of proteome-informative, protein
N-terminal peptides by combined fractional diagonal chro-
matography (COFRADIC). Proteomics 2008, 8, 1362–1370.
[17] Gevaert, K., Van Damme, J., Goethals, M., Thomas, G. R.
et al., Chromatographic isolation of methionine-containing
peptides for gel-free proteome analysis: identification of
more than 800 Escherichia coli proteins. Mol. Cell. Proteo-
mics 2002, 1, 896–903.
[18] Godon, C., Lagniel, G., Lee, J., Buhler, J. M. et al., The H2O2
stimulon in Saccharomyces cerevisiae. J. Biol. Chem. 1998,
273, 22480–22489.
[19] Kusch, H., Engelmann, S., Albrecht, D., Morschhauser, J.,
Hecker, M., Proteomic analysis of the oxidative stress
response in Candida albicans. Proteomics 2007, 7, 686–697.
[20] Gerth, U., Kock, H., Kusters, I., Michalik, S. et al., Clp-
dependent proteolysis down-regulates central metabolic
pathways in glucose-starved Bacillus subtilis. J. Bacteriol.
2008, 190, 321–331.
[21] Dixon, D. P., Skipsey, M., Grundy, N. M., Edwards, R.,
Stress-induced protein S-glutathionylation in Arabidopsis.
Plant Physiol. 2005, 138, 2233–2244.
[22] Meisenhelder, J., Hunter, T., Radioactive protein-labelling
techniques. Nature 1988, 335, 120.
[23] Jehmlich, N., Schmidt, F., von Bergen, M., Richnow, H. H.,
Vogt, C., Protein-based stable isotope probing (Protein-SIP)
reveals active species within anoxic mixed cultures. Isme
J. 2008, 2, 1122–1133.
[24] Schmidt, F., Scharf, S. S., Hildebrandt, P., Burian, M. et al.,
Time-resolved quantitative proteome profiling of host-
pathogen interactions: the response of Staphylococcus
aureus RN1HG to internalisation by human airway epithe-
lial cells. Proteomics 2010, 10, 2801–2811.
[25] Keller, A., Purvine, S., Nesvizhskii, A. I., Stolyar, S. et al.,
Experimental protein mixture for validating tandem mass
spectral analysis. Omics 2002, 6, 207–212.
[26] Nesvizhskii, A. I., Keller, A., Kolker, E., Aebersold, R., A
statistical model for identifying proteins by tandem mass
spectrometry. Anal. Chem. 2003, 75, 4646–4658.
[27] Roeser, J., Bischoff, R., Bruins, A. P., Permentier, H. P.,
Oxidative protein labeling in mass-spectrometry-based
proteomics. Anal. Bioanal. Chem. 2010, 397, 3441–3455.
[28] Paley, S. M., Karp, P. D., The pathway tools cellular over-
view diagram and omics viewer. Nucleic Acids Res. 2006,
34, 3771–3778.
[29] Kim, Y. H., Cho, K., Yun, S. H., Kim, J. Y. et al., Analysis of
aromatic catabolic pathways in Pseudomonas putida KT
2440 using a combined proteomic approach: 2-DE/MS and
cleavable isotope-coded affinity tag analysis. Proteomics
2006, 6, 1301–1318.
[30] Kurbatov, L., Albrecht, D., Herrmann, H., Petruschka, L.,
Analysis of the proteome of Pseudomonas putida KT2440
grown on different sources of carbon and energy. Environ.
Microbiol. 2006, 8, 466–478.
[31] Reva, O. N., Weinel, C., Weinel, M., Bohm, K. et al., Func-
tional genomics of stress response in Pseudomonas putida
KT2440. J. Bacteriol. 2006, 188, 4079–4092.
[32] Jimenez, J. I., Minambres, B., Garcia, J. L., Diaz, E., Geno-
mic analysis of the aromatic catabolic pathways from
Pseudomonas putida KT2440. Environ. Microbiol. 2002, 4,
824–841.
42 N. Jehmlich et al. Proteomics 2012, 12, 37–42
& 2011 WILEY-VCH Verlag GmbH & Co. KGaA, Weinheim www.proteomics-journal.com