endocytic trafficking during drosophila development
TRANSCRIPT
Endocytic trafficking during Drosophila development
Marcos Gonzalez-Gaitan
Max-Planck Institute for Molecular Cell Biology and Genetics, Pfotenhauerstr. 108, Dresden D-01307, Germany
Accepted 12 June 2003
Abstract
During the last decade, many of the factors and mechanisms controlling membrane and protein trafficking in general and endocytic
trafficking in particular have been uncovered. We have a detailed understanding of the different endocytic trafficking steps: plasma
membrane budding, endocytic vesicle motility and fusion with the endosome, recycling, transcytosis and lysosomal degradation. The
kinetics and trafficking pathway of many signaling receptors and the relevance of endocytic trafficking during signaling in many mammalian
cultured cells are also well understood. However, only in recent years has the role of endocytic trafficking during cell-to-cell communication
during development, i.e. during patterning, induction and lateral inhibition, begun to be explored. The contribution of Drosophila
developmental genetics and cell biology has been fundamental in elucidating the essential role of endocytosis during these processes.
Reviewed here are some of the recent developments on the role of endocytic trafficking during long- and short-range signaling and during
lateral inhibition.
q 2003 Elsevier Ireland Ltd. All rights reserved.
Keywords: Endocytic trafficking; Morphogenetic signaling; Morphogens; Decapentaplegic; Wingless; Hedgehog; Notch; Delta
1. Endocytic trafficking during long-range
morphogenetic signaling: Dpp in the wing
1.1. Organizers and long-range morphogens
During morphogenesis, cells within developing tissues
acquire positional information in a process that involves a
particular kind of signaling molecules: the morphogens
(Turing, 1952; Wolpert, 1969). Morphogens are ligands
which are secreted from a restricted groups of cells, a
source. Upon secretion, morphogens move away from the
source to form gradients of concentration. Positional
information is encoded in the graded distribution of
morphogens: cells read their distance to the source by
computing the morphogen concentrations which surround
them. Long-range morphogens act as organizers, being
secreted from a small source and providing positional
information to cells far away from the producing cells.
Therefore morphogens move far from their source and
establish a stable gradient that lasts during several days of
development. What cellular mechanisms control the long-
range movement of morphogens? What ensures their graded
distribution? How are their slopes and ranges stably
maintained?
To answer these questions it is necessary to know: (i) the
key factors involved in the morphogenetic signaling event,
i.e. the signaling cascade from the ligand, through the
receptor and the effecting transcription factors; (ii) the
developmental properties of the signaling event: where is
the source? which are the receiving cells? which target
genes are activated at which distance from the source? and
(iii) how developing cells (as opposite to cultured cells)
control membrane and protein trafficking at the molecular
level and establish the kinetic parameters of protein
movements within and between cells in the tissues where
morphogenetic signaling is taking place. This rich pool of
interdisciplinary information is starting to be available in
the case of morphogenetic signaling in Drosophila. In
particular, the role of endocytic trafficking in three
morphogenetic signaling pathways, Dpp, Wingless and
Hedgehog, are the focus of a number of Drosophila
laboratories in recent years. The comparison of the role of
endocytosis during these three signaling events uncovers
how endocytic trafficking mediates long-range signaling
(Dpp) as well as shorter signaling events (Wg, Hh).
0925-4773/$ - see front matter q 2003 Elsevier Ireland Ltd. All rights reserved.
doi:10.1016/j.mod.2003.06.002
Mechanisms of Development 120 (2003) 1265–1282
www.elsevier.com/locate/modo
E-mail address: [email protected] (M. Gonzalez-Gaitan).
1.2. Dpp and endocytosis: spreading by planar transcytosis
Dpp acts as a long-range morphogen that provides
information along the anterior–posterior axis during wing
development (Capdevila et al., 1994). Dpp directly
activates the expression of target genes in a concentration
dependent manner (Lecuit et al., 1996; Nellen et al., 1996).
Thus, two target transcription factors, the zinc-finger
proteins Spalt and Optomotorblind are expressed in nested
domains of expression around the Dpp expressing cells
during wing development. Dpp forms a gradient spanning
40 cells diameters that activates Spalt in wing cells at a
distance of 15 cells and Omb as far as 30 cells away from
the source.
Dpp spreading to form such a long-range gradient
requires endocytosis at the receiving cells (Entchev et al.,
2000; Gonzalez-Gaitan and Jackle, 1999). Three kind of
experiments uncovered the role of endocytosis during long-
range movement of Dpp: the ‘shibire rescue’ assay, the
‘shadow’ assay and the receptor mosaic assay (Fig. 1A–D)
(Entchev et al., 2000). In a set of experiments (shibire
rescue; Fig. 1B), endocytosis was blocked in the receiving
cells using the thermosensitive Dynamin mutant shibire,
while the producing cells at the source were rescued by
expressing there a Dynamin transgene. In these developing
wings, fluid phase endocytosis was controlled by observing
dextran internalization into endosomes: endocytosis was
restricted to the source of Dpp and internalization was
tightly blocked in the receiving cells. In this scenario, Dpp
internalization into endosomes was blocked in the receiving
cells and its distribution was reduced to the first three cell
rows adjacent to the source, where it appeared as an
extracellular weak staining. These observations suggested
that long-range spreading requires Dpp endocytosis by the
receiving cells. It is, however, still possible that extra-
cellular Dpp is diluted in a larger volume than the
endosomes: low levels of Dpp would only be visible when
concentrated in the endosomes.
The shadow assay, however, shows that indeed endocy-
tosis is essential during long-range Dpp trafficking (Fig. 1C).
In the shadow assay, the progression of Dpp emanating from
the source is challenged by a patch of shibire mutant cells
which cannot perform endocytosis. The assay takes
advantage of the thermosensitivity of Dpp expression
driven by the gal4 system and the thermosensitivity of
shibire. The experiment starts at low temperature, when
(i) the shibire cells can perform endocytosis at the
permissive temperature and (ii) low levels of Dpp are
expressed and therefore it cannot be seen in the receiving
cells. Then, raising the temperature has two consequences:
(i) endocytosis is blocked in the patch of shibire cells; (ii) a
wave of Dpp secreted from the source is travelling through
the tissue. When confronted with the shibire clone of cells
the wave of Dpp cannot cross the endocytosis defective
tissue and therefore a shadow with low levels of Dpp is
formed distal to the mutant mosaic. The shadow is,
however, transient because Dpp moves rapidly and in all
directions, entering shortly thereafter (within few hours) the
shadow area.
The Dpp receptor, composed of two proteins, Punt and
Thickveins (Tkv), is required for Dpp internalization and for
its long-range movement. A patch of Tkv mutant cells is
incapable of internalizing Dpp. As a consequence Dpp
accumulates around the mutant cells. But extracellular Dpp
accumulation is restricted to the cells of the clone which
face the Dpp source (Fig. 1D). An explanation of this
behaviour of the Tkv clone is that Dpp accumulated around
the cells facing the source is unable to progress further into
the mutant territory, suggesting again a scenario in which
Dpp movement through the target tissue requires its
internalization by endocytosis, specifically by Dynamin-
dependent receptor-mediated endocytosis.
Based on these three observations, a planar transcytosis
model has been proposed in which Dpp movement through
the target tissue involves short-range extracellular diffusion
(across less than 3 cell diameters) and active transport of the
morphogen through the receiving cells by vesicular
trafficking involving the endocytosis and re-release of the
morphogen molecules (Fig. 1E) (Entchev et al., 2000). In
this scenario, endocytic block allows the short-range
extracellular diffusion of the morphogen, but impedes its
active transport through the cells and thereby its long-range
distribution in the tissue.
1.3. An alternative model: Dpp spreading by diffusion
The above three assays show that the control of receptor-
mediated endocytosis is required in order to achieve the
long-range spreading of Dpp. The planar transcytosis model
assumes that Dpp internalized in the receiving cells is re-
secreted to be internalized (and signal) in the neighbouring
cells. The event of Dpp re-secretion from the receiving cells
has, however, not yet been directly monitored. Therefore, an
alternative formal possibility is that internalization is not
required as the first step of Dpp planar transcytosis, but that
endocytosis down-regulates another critical molecule by
removing it from the plasma membrane. Thus it has been
suggested that endocytosis block causes the accumulation of
the Dpp receptor at the cell surface and this in turn traps Dpp
while moving extracellularly by free-diffusion across the
extracellular matrix (Fig. 2A) (Lander et al., 2002). This
possibility is supported by the fact that Dpp signaling range
is decreased by overexpression of the receptors at the
receiving cells (Lecuit and Cohen, 1998). In this scenario, a
proper internalization of the receptor ensures that enough
Dpp free molecules could circulate to build-up the long-
range gradient. To address this possibility, the differential
equations governing Dpp trafficking by free-diffusion
through the extracellular space were studied (Fig. 2B)
(Lander et al., 2002). The model of Lander et al. assumes:
(i) extracellular diffusion of Dpp according to the Fick’s
law; (ii) binding/release of Dpp to the receptors at the plasma
M. Gonzalez-Gaitan / Mechanisms of Development 120 (2003) 1265–12821266
membrane; (iii) endocytosis, recycling and degradation of
the free receptors and endocytosis þ degradation of the
ligand bound to the receptors; (iv) boundary conditions in
the modeling area: Dpp is degraded in a sink region of
the developing tissue and (v) before GFP-Dpp emanates
from its source, there is no Dpp in the receiving tissue.
In the model, the developing wing is simplified in its
geometry to a one-dimensional diffusion problem in which
Fig. 1. Experimental assays to study the role of endocytosis during Dpp morphogen movement. (A) Dpp long-range gradient. Dpp forms a gradient of
concentration from the source, (red cells, left) and appears graded both extracellularly and when internalized in the endosomes. (B) ‘Shi rescue assay’. It
consists of mosaic discs where the producing cells at the source (red cells, left) are wildtype (shiþ) while the receiving cells (right) are mutants for a
thermosensitive mutation in Dynamin (shits) and thereby endocytosis defective cells. Endocytosis is blocked for 6 h. Dpp, degraded, disappears from the
endosome of receiving cells, while extracellular Dpp is restricted to the cells adjacent to the source. (C) ‘Shadow assay’. It starts by producing a tissue void of
Dpp at the receiving cells. A patch of shits cells is generated at the permissive temperature. Then Dpp is pulsed from the source and endocytosis is blocked at the
restrictive temperature of shits. The front of Dpp advancing through the tissue meets the mutant clone. It cannot move across the endocytosis defective territory
and forms a shadow behind the clone. (D) ‘Receptor mosaic assay’. Consist in a mutant clone that lacks the receptor. The clone is exposed to the gradient for
many cell generations. As a consequence, Dpp, which cannot be internalized by receptor-mediated endocytosis, accumulates in between the cells of the clone
which are nearer the source. (E) A model of Dpp spreading by planar transcytosis. Dpp is secreted to an apical location below the adherens junctions from the
producing cells. At the extracellular space, it does not move a long distance by simple diffusion. Instead it is internalized by endocytosis and accumulates in an
apical endosome from where it is degraded or recycled again. This way it moves on through the next cells and thereby spreads through the target tissue forming
a gradient. Degradation in each of the receiving cells ensures the formation of a stable gradient of concentration.
M. Gonzalez-Gaitan / Mechanisms of Development 120 (2003) 1265–1282 1267
Fig. 2. Modelling the free-diffusion of morphogens. (A) Endocytosis block may cause surface receptor accumulation. (i) Internalization of receptors (II)
by endocytosis regulates the amount of surface receptors at the plasma membrane. Receptors internalized by endocytosis are targeted to degradation.
Receptors at the plasma membrane bind to the morphogen (green) and hamper its further spreading through the target tissue. (ii) In endocytosis defective
cells (grey cells) surface receptors are not down-regulated by endocytosis, thereby causing accumulation of receptors at the plasma membrane.
Accumulated at the plasma membrane, high levels of receptors block the progression of the morphogen through the receiving cells. (B)
Parameters affecting the free-diffusion of morphogens when surface receptors hamper their spreading. (C) System of differential equations which describes
the free-diffusion and titration of morphogen spreading by surface receptors. (D–F) Behaviour of the shadow assay under a model of free-diffusion of the
morphogen and spreading is impaired by surface receptors. (D) Internalized Dpp in the shadow assay (gray, shibire-clone) before the steady-state (5 h).
Note that a shadow is seen behind the clone (i), but also before the clone (ii). Also note that, in the clone where internalization is blocked internalized
Dpp is increased (iii). This is due to the fact that the levels of extracellular receptors are 10 times those of the wildtype situation and endocytosis is not
M. Gonzalez-Gaitan / Mechanisms of Development 120 (2003) 1265–12821268
the morphogen is introduced at a rate n at one location (the
source), and absorbed at another, a sink at the edge of the
gradient where the morphogen is totally degraded. While it is
clear that there is a source of Dpp in the developing wing, no
sink exists in the developing wing primordium, i.e. no region
in the disc is dedicated to the total degradation of the
remaining morphogen. The existence of such sink by itself
would generate gradients resembling the one observed for
Dpp regardless of the mechanism of transport proposed.
Within the modeling area, diffusion of Dpp would
behave according to Fick’s second law
›½L�=›t ¼ D›2½L�=›x2
where ½L� is the concentration of the morphogen, t is time, x
is distance and D the diffusion coefficient. In addition to
this, Dpp spreading is governed by Dpp/receptor binding
and dissociation (with constants kon and koff, respectively) as
well as the rates of biosynthesis, endocytosis and degra-
dation of the receptor and the receptor/ligand complexes
(Fig. 2B,C). Then, the receptor/ligand association rate
constant (kon ¼ 3 £ 105 or 1.2 £ 105 M21 s21) is introduced
from the literature (Iwasaki et al., 1995; Natsume et al.,
1997). The values of the other parameters were scanned to
fit the gradient shape and kinetics of gradient formation
observed for Dpp. The values of the different trafficking
rates selected this way were smaller than those previously
estimated experimentally for EGF and its receptor (Lauf-
fenburger and Linderman, 1993). This analysis shows that
there is a universe of parameters for which a gradient
resembling that observed for Dpp can be formed by
extracellular diffusion and receptor binding.
Lander et al. argued that another interesting conse-
quence of the model is that in a scenario of diffusion and
receptor binding as proposed by their model, shibire
clones would also generate distal shadows. This is due to
the fact that endocytosis block would cause the accumu-
lation of surface receptors at the shibire mutant cells
thereby trapping Dpp on its travel to form the gradient
(Fig. 2D–F). However, in the model, both the shadow and
the clone behave different from the experimentally
observed situation: (i) surprisingly shadows can be seen
distally (Fig. 2Di), but also proximally to the shibire clone
(Fig. 2Dii); (ii) the result of blocking internalization in the
clone is that the internalized Dpp is increased with respect
to wildtype cell (Fig. 2Diii), which was not observed in
the shibire clones: internalized Dpp disappeared in the
endocytosis-defective cells, it was not increased! and (iii)
the amount of extracellular Dpp at the clone increased by
a factor of 40 (Fig. 2Eiv), which was also not observed.
In summary, the shibire clone in a scenario of diffusion þ
receptor binding of Dpp behaves different to the observed
result (cf. Figs. 2G vs. 1B).
In addition, in the simulation of the shibire clone, in the
endocytosis defective cells, the receptor levels increase by a
factor of 10 instantaneously, instead of increasing progress-
ively according to the differential equations and the
biosynthetic rates proposed when endocytosis is blocked
in the shibire clone. As a consequence, when the Dpp
propagation front reaches the clone, it finds a concentration
of the receptor 10 times bigger than normal causing the
formation of the shadow behind. After 6 h of endocytic
block, the levels of the Dpp receptor determined exper-
imentally using antibodies do not increase by a factor of 10,
but only suffer a marginal increase (Pantazis and G-G,
unpublished results).
Another issue is the plausibility of the spreading of Dpp
by intracellular trafficking. It has been argued that if moving
by intracellular trafficking, Dpp has to be transported across
a single cell in 150 s on average in order to account for the
speed of expansion of the Dpp gradient in less than 8 h. For
various mesenchymal cells in culture, the rates of recycling
of ligands such as Transferrin or EGF imply mean transit
times of minutes to hours (Sheff et al., 1999; Shitara et al.,
1998). No data is, however, available in the case of
developing epithelial cells. Interestingly, secretion to the
apical-junctional complex in MDCK cells mediated by the
exocyst (Grindstaff et al., 1998) and accumulation of
receptors to the junctional region (Banerjee et al., 1987;
Fehon et al., 1991; Tomlinson et al., 1987) may make the
transport from cell to cell more effective than the three-
dimensional random walk predicted by Fick’s law which is
on the basis of the model. It is worth noting that Dpp
accumulates in apical endosomes (Entchev et al., 2000),
also suggesting that the trafficking routes of Dpp in the
developing epithelial wing cells might be far from random
throughout the full volume of the cell. It will be interesting
to estimate experimentally the rates of dissociation of Dpp
from its receptor and, more generally, its trafficking routes
and kinetics at the receiving cells. In the future, a
fluent crosstalk between experimental data and modeling
of non-linear systems will be necessary in order to integrate
trafficking and developmental approaches.
1.4. Endosomal dynamics during Dpp signaling
Trafficking through the endocytic pathway involves a
number of intermediate compartments, including the early
endosome, where the decision is made to target the endocytic
totally blocked in the simulation, but decreased by a factor of 10. Therefore, although endocytosis is decreased, the huge amount of surface receptors
account for increased receptor-mediated endocytosis inside the clone. This was not seen in the experimental data. (E) Surface Dpp in the shadow assay
(gray, shibire-clone) before the steady-state (5 h). Surface Dpp is increased by a factor of 40 (iv). (F) Internal Dpp after 24 h. No shadow can be seen.
This, however, does not represent the steady-state situation. (G) Schematic representations of the behaviour of the shadow assay in the diffusion/
hampering receptors model. The result differs substantially from the observed results (cf. Fig. 1C).
R
M. Gonzalez-Gaitan / Mechanisms of Development 120 (2003) 1265–1282 1269
cargo to recycling or to degradation at the late endosome/-
lysosome (reviewed in Mukherjee et al., 1997). Each
particular trafficking step through the endocytic pathway
is controlled by a small GTPase of the Rab family. Thus,
Rab5 controls the step from the plasma membrane to the
early endosome, Rab7 controls the targeting to the
degradation pathway and Rab4/Rab11, the recycling path-
way (reviewed in Novick and Zerial, 1997). Consistent with
their role in endosomal dynamics, these Rab proteins accu-
mulate in distinct endosomal compartments: Rab4/Rab5 in
the early endosome, Rab11 in a recycling endosome and
Rab7 in the late endosome. In Drosophila, these factors are
highly conserved in aminoacid sequence (between 75 and
85% identity, 83–91% similarity), localization and function
(Entchev et al., 2000 and unpublished results).
The mutant phenotype of these Rab proteins and their
localization with respect to Dpp uncovered an essential
role of endosomal dynamics during Dpp signaling
(Entchev et al., 2000). Thus, blocking Rab5 in the
receiving cells causes a reduction of Dpp signaling range,
as monitored by the distance to the source at which
target genes are activated. Conversely, Rab5 overexpres-
sion causes an expansion of the Dpp signaling range
(Fig. 3C). Similarly, enhanced degradation caused by
expression of a gain of function Rab7 mutant protein in
the receiving cells reduces the signaling range.
These results are consistent with a scenario in which
internalized Dpp is directed to degradation and recycling in
the receiving cells in a mechanism controlled by Rab
proteins which determines the efficiency of Dpp spreading
and thereby the range and slope of the gradient. In addition
to controlling Dpp spreading, endosomal dynamics may
also determine the efficiency of Dpp signal transduction.
Indeed, endosomal trafficking turned out to critically control
the signal transduction event by other TGF-beta-like ligands
in mammalian cells.
1.5. TGF-beta signal transduction and endosomal dynamics
in mammalian cells: SARA, Smurfs, Clathrin and Caveolin
TGF-beta signals through heteromeric complexes of Type
II and Type I transmembrane Ser-Thr kinase receptors
(reviewed in Massague, 1998). Ligand induces the assembly
of a heteromeric receptor complex within which Type II
receptor transphosphorylates and activates the Type I
receptor (Wrana et al., 1994). The Type I receptor in turn
phosphorylates the receptor regulated Smads, R-Smads
(Smad1,2,3,5,8) (Miyazono, 2000). Once phosphorylated,
the R-Smads bind to another Smad, the Co-Smad Smad4,
forming a complex which is imported in the nucleus
and elicits transcription of target genes. Finally the inhibitory
Smads, I-Smad (Smad6,7), negatively regulate TGF-beta
signaling by binding to the Type I receptor and recruiting the
Smurf E3 ubiquitin ligases, which direct the ubiquitin-
dependent degradation of the TGF-beta receptor–Smad7
complexes (Ebisawa et al., 2001; Kavsak et al., 2000).
Like other receptors, the TGF-beta receptors are
down-regulated by internalization both constitutively
and upon ligand binding (Massague and Kelly, 1986;
Sathre et al., 1991). Endocytosis here may affect
negatively the signal transduction event by removing
the receptors from the plasma membrane where the
ligand binds the receptors and the receptors phosphor-
ylate the transcription factor. The discovery of an
endosomal protein, SARA, as an essential adaptor
between the activated Type I receptor and the transcrip-
tion factors, Smad2/3, uncovered the endosome as a
platform during signal transduction (Tsukazaki et al.,
1998). In mammalian cells, SARA acts specifically
during Smad signaling involving Smad2/3 which mediate
TGF-beta/Activin signaling, but not Smad1/5/8 which
mediate BMP signaling (Tsukazaki et al., 1998). In
Drosophila, however, it has been suggested that Droso-
phila SARA is also involved in Dpp signaling, a BMP
pathway mediated by an Smad1 homolog, Mad (Bennett
and Alphey, 2002).
SARA is targeted to the endosome through its FYVE
finger domain (Hayes et al., 2002; Itoh et al., 2002;
Panopoulou et al., 2002), which specifically binds to PI(3)P
when in a bilayer, a situation specific of the early endosomal
membrane and the internal vesicles of the multivesicular
bodies (Gillooly et al., 2000). In addition to its role as an
adaptor, SARA itself is involved in endosomal dynamics in
a process that also requires its FYVE domain (Hayes et al.,
2002; Itoh et al., 2002; Panopoulou et al., 2002), reminiscent
of other FYVE domain proteins such as EEA1 and
Rabenosyn which are involved in endocytic vesicle
tethering and fusion with the endosome (Gillooly et al.,
2001; Wurmser et al., 1999).
What role does SARA play during Smad phosphoryl-
ation? Three possibilities have been proposed: (i) targeting
of Smad to the receptor when localized at the endosome, (ii)
Smad phosphorylation at the endosome and (iii) diversion of
activated receptors away from the degradation pathway.
Based on the fact that SARA binds directly to the Type I
receptor and Smad2 it was proposed that SARA acts by
targeting Smad to the receptor. This event would take place
at the endosome, mediated by the targeting of SARA itself
to this compartment by means of its FYVE domain (Fig. 3D)
(Tsukazaki et al., 1998). However, if endocytosis is blocked,
SARA is still found in a trimeric complex with the receptor
and Smad2, suggesting that this interaction does not need
the endosomal milieu (Penheiter et al., 2002). While
the trimeric complex forms at the plasma membrane,
phosphorylation of Smad2 by the Type I receptor is blocked
in the absence of endocytosis, suggesting that SARA
endosomal localization is essential to allow Smad2
phosphorylation.
An interesting model for the role of the endocytic
pathway during TGF-beta signal transduction has been
suggested recently by the Wrana Laboratory, which
originally discovered SARA (Fig. 3E) (Di Guglielmo et al.,
M. Gonzalez-Gaitan / Mechanisms of Development 120 (2003) 1265–12821270
2003; Tsukazaki et al., 1998). They showed that TGF-beta
receptors internalize both into Caveolin- and EEA1-positive
vesicles. These vesicular structures are the target compart-
ments of the endocytic vesicles generated by two different
molecular mechanisms: Clathrin-mediated endocytosis
generates EEA1-positive vesicles and caveolae, deep
invaginations of the membrane, generate vesicular struc-
tures containing the raft-protein Caveolin. Rafts are lipid
microdomains enriched in cholesterol which has been
proposed to play an essential role as signaling platforms
(Simons and Ikonen, 1997). However, in the case of TGF-
beta signaling, it seems that the Clathrin dependent
internalization of the receptors into the EEA1-positive
endosome, where the Smad2 anchor SARA is enriched,
promotes TGF-beta signaling, while the lipid raft-caveolar
internalization pathway is required for rapid receptor
degradation. Thus, in the Caveolin-positive compartment
the receptor colocalizes with Smad7–Smurf2, two factors
Fig. 3. Role of endocytic trafficking during TGF-beta-like signaling. (A–C) Essential and rate-limiting role of Rab5 during Dpp signaling. (A) Wild-type. Dpp
emanating from the source (green cells) activates target genes such as Spalt at a distance from the source (red cells). (B) Dominant negative Rab5 mutant in the
posterior receiving cells (dash) reduced the range of Dpp signaling: only cells adjacent to the source activate the target gene. (C) Rab5 overexpression in the
posterior receiving cells expands the range of Dpp signaling. To drive the mutant Rab5 proteins the Engrailed-gal4 driver (en < ) was used. A/P,
anterior/posterior boundary. Arrows represent the range of Dpp signaling. (D) Model of SARA-mediated TGF-beta signal transduction from the endosome.
Binding of TGF-beta to the receptor at the plasma membrane causes phosphorylation of the Type I receptor and activation of its kinase. At the endosome,
SARA brings the Smad2 transcription factor to the receptor. Then Smad2 is phosphorylated and becomes active and imported into the nucleus. (E) A model of
endosome/caveolae competition for TGF-beta signaling. CCP, Clathrin-coated pit. For details, see text.
M. Gonzalez-Gaitan / Mechanisms of Development 120 (2003) 1265–1282 1271
Fig. 4. Endocytosis, lysosomal degradation and asymmetric Wg signaling. (A–E) Embryonic segmentation of the cuticle involves four different signaling
pathways. (A) Stages 9 and 10. Mutual activation of Wg (red) and Hh (blue) in adjacent cells. Wg is distributed symmetrically at both sides of its source.
(B) Stage 11. Ser (grey) is expressed between the Hh and Wg stripes due to repression from both signaling pathways. Wg is already distributed asymmetrically.
(C) Stage 12. Rho (green) is expressed in the cells between Hh and Ser. This is because either ligand can activate Rho expression. Anterior to Hh and posterior
to Ser, Rho is not expressed due to repression by Wg. (D) Spi (green) is secreted from the Rho expressing cells and activate the expression of Svb (orange), the
master regulator of denticle differentiation. Spi activates Svb expression in a longer range towards anterior than towards posterior. This is due to long-range
M. Gonzalez-Gaitan / Mechanisms of Development 120 (2003) 1265–12821272
which are involved in receptor degradation and signaling
down-regulation. Thus, segregation of TGF-beta receptors
into distinct endocytic compartment regulates Smad acti-
vation and receptor turnover mediated by Smurf.
Smurf proteins are E3 ubiquitin ligases that inhibit TGF-
beta signaling and ubiquitinate both the TGF-beta receptors
and Smad proteins (Kavsak et al., 2000; Lin et al., 2000;
Zhu et al., 1999). Consistently, a Drosophila Smurf
mutation is unable to inhibit Dpp signaling and expands
indeed the signaling range (Podos et al., 2001). Smurf
proteins seem to act at three levels during TGF-beta
signaling inhibition: (i) ubiquitination of the R-Smads to
target it to the proteosome for degradation (Lin et al., 2000;
Zhu et al., 1999); (ii) binding to the I-Smad Smad7 to target
it to the receptor where it competes with the R-Smad for
receptor binding (Ebisawa et al., 2001; Kavsak et al., 2000)
and (iii) target the receptor–Smad7 complex for degra-
dation a process that at least partially takes place in the
lysosome, thereby down-regulating the receptor (Kavsak
et al., 2000).
2. Endocytic trafficking during short-range
morphogenetic signaling: Wg in the embryo
While Dpp signals over a long-range during wing
development across 40 cell diameter, other signaling
molecules, like Wingless, are also distributed as a gradient,
but with a short-range. During embryogenesis, the Wg
signal extends across 4 cell diameters in the developing
epidermis. While it is not clear whether Wingless acts itself
as a morphogen (Martinez Arias, 2003), its distribution as a
gradient and/or its signal transduction mechanism seems
also to be mediated by endocytic trafficking. The role of
endocytosis during Wingless signaling was best studied
during segmentation (Fig. 4A–G).
2.1. Segmentation: an array of signaling molecules
and the asymmetric spreading of Wg
Drosophila larval epidermis shows a repetitive pattern of
cuticular structures that manifest the segmental organization
of the insect body (Fig. 4E). Each epidermal segment
derives from a stripe of 12 rows of embryonic cells. On the
ventral surface of the larva, cell rows 1–5 and 12
differentiate denticles which are small hair-like structures
at the apical side of the epidermal cells, while cell rows
6–11 show a smooth surface also called ‘naked cuticle’
(Fig. 4E). During embryonic segmentation, four different
signaling pathways, (Hedgehog (Hh), Wingless (Wg),
Notch (N) and EGF-receptor) interact with one another to
give rise to the spatial information which lies on the basis of
this stereotyped spatial distribution of cuticular elements.
Early during embryogenesis, Hh and Wg are expressed in
adjacent stripes of cells (Fig. 4A). At this time, Hh and Wg
are involved in a paracrine signaling loop: Hh activates
expression of Wg in the adjacent cells and vice versa
(DiNardo et al., 1988; Ingham et al., 1988). In addition, both
Hh and Wg repress expression of a third signaling molecule,
the Notch ligand Serrate (Ser) which is thereby expressed in
the middle of the segment (rows 4–6) where neither Hh
(rows 11,12) nor Wg (row 10) reach (Fig. 4B) (Alexandre
et al., 1999; Wiellette and McGinnis, 1999). Finally a fourth
ligand, the EGF-receptor ligand Spitz, is secreted from a
stripe of cells (rows 1–3) between Hh and Ser. Restricted
secretion of Spitz is mediated by Rhomboid (Rho), which is
expressed in these cells (Golembo et al., 1996). Rho
expression is activated by both Hh and Ser and repressed by
Wg, hence the localization of the Rho stripe and restricted
Spitz secretion (Fig. 4C) (Alexandre et al., 1999; Gritzan
et al., 1999; Sanson et al., 1999).
A single master transcription factor, Shavenbaby (Svb),
controls the differentiation of the denticles in the cell rows
12/1–5 (Payre et al., 1999). Svb expression is activated by
Spitz emanating from rows 1–3 and repressed by Wg
secreted from row 10 (Fig. 4D). Wg spreading from row 10
is asymmetric, with a range of four rows towards anterior
and only one cell row towards posterior. This explains the
skewed localization of Svb at both sides of the Spitz
secreting cells. Therefore, positional information is deter-
mined in this case by an array of signaling molecules
arranged in a spatial sequence and by the asymmetric range
of spreading of one of the ligands, Wg.
2.2. Asymmetric wingless signaling in the embryo:
asymmetric degradation
Wg is distributed symmetrically at the beginning of
embryogenesis (Fig. 4A) and its posterior range of
spreading is restricted later (Fig. 4B–D) (Gonzalez et al.,
1991). Secreted Wg seems to be stabilized by its receptors at
the anterior side, since posterior restriction correlates with a
posterior reduction of the RNA levels of Wg receptors,
Frizzled and Frizzled2 (Dubois et al., 2001). Another level
repression of Svb by wingless towards anterior and short Wg repression towards posterior. As a consequence Rho expression domain is not centered with
respect to Svb. (E) Differentiation of denticles depends on Svb which is due to the interplay of four signaling pathways (Wg, Hh, Rho, Ser) distributed in an
array of cells along the anterior–posterior axis. Positioning of Svb depends on Rho/Spi and asymmetric signaling by Wg. 1–12, cell rows within the segmental
unit (delimited by vertical lines). (F) Secreted Wg is internalized into in an early endosomal structure. Wg is degraded in a lysosome where it could not be
detected. Its distribution is asymmetric. (G) HRP-Wg reveals the asymmetric degradation of Wg. HRP-Wg is symmetrically distributed. Due to the HRP
moiety, it can be detected both in the early endosome and the lysosome. It therefore uncovers enhanced lysosomal degradation in the posterior cells. As a
consequence it shows a symmetric distribution: HRP-Wg in early endosomes of anterior cells; HRP in the lysosomes of posterior cells. In posterior cells,
enhanced degradation is controlled by Spi signaling (green dots) emanating from Rho expressing cells (green nuclei).
R
M. Gonzalez-Gaitan / Mechanisms of Development 120 (2003) 1265–1282 1273
of regulation for the posterior spreading of Wg is its specific
degradation at the lysosome: Wg is degraded at higher rates
in the posterior cells than in the anterior ones (Dubois et al.,
2001).
This was shown by monitoring a functional horseradish
peroxidase (HRP)-Wgfusion(Duboisetal.,2001).HRPin the
fusion persists in the lumen of the degradative compartment
even after Wg itself has been digested. At a stage when Wg
already spreads asymmetrically from row 10 and is only seen
in the posterior cells adjacent to the source (Fig. 4F), HRP-
wingless shows a symmetric distribution and can be seen in
posterior cells distant from the source (Fig. 4G). Therefore,
the posterior restriction of Wg requires its differential
degradation in posterior cells (Fig. 4F,G). At the EM level,
HRP-Wg is indeed seen in degradative compartments:
multivesicular (MVB) and multilamellar bodies (MLB), con-
firming previous immuno-EM results (Gonzalez et al., 1991;
vandenHeuveletal.,1989).AlthoughMVB/MLBcontaining
HRP-Wg are seen in both anterior and posterior cells, Wg
seems to be more actively degraded in the posterior cells,
since HRP-Wg-labelled MVB/MLB in the posterior cells are
four times more frequent than in anterior cells.
Consistent with the idea that the asymmetric distribution
of Wg is mediated by its differential degradation, treatment
with chloroquine, a lysosomal inhibitor, or reduction of
internalization by endocytosis and lysosomal degradation
with Clathrin heavy chain and deep orange mutations
abolishes the asymmetric distribution of Wg (Dubois et al.,
2001). How is this differential degradation controlled?
Restricted Wg spreading towards posterior is under the
control of Hh: in Hh pathway mutants, Wg distribution
remains symmetric (Sanson et al., 1999). As described above,
Hh activates Rho expression inposterior cells determining the
restrictedsecretionof the EGF-receptor ligand Spitz,which in
turn elicits the transcription of an unknown factor mediating
enhanced Wg degradation in the cells that received the Spitz
signal (Fig. 4G). Ina numberofcases,EGF-receptor signaling
has been shown to control endocytic trafficking by interfering
with the Rab5 endocytic machinery (Lanzetti et al., 2000; Tall
et al., 2001), suggesting this small GTPase and its regulators/
effectors as possible targets of Spitz control.
2.3. Endocytosis and Wg signaling
What signaling step is affected by the differential
degradation of Wg? Spreading? Transduction? The fact
that HRP-Wg is seen far from the source in the posterior
cells, suggests that Wg spreading is not affected by
differential degradation. An alternative possibility is that
Wg signal transduction is affected by the degradation of Wg.
Future work will elucidate which of this two possibilities are
more plausible, and whether wg signal transduction occurs
from an intracellular locale.
Wg is internalized by Dynamin-mediated endocytosis
into vesicular structures in the target tissue (Bejsovec and
Wieschaus, 1995). In shibirets mutants, Wg is only able to
elicit signaling in cells adjacent to row 10. Therefore,
long-range Wg activity requires endocytosis. Again, is
endocytosis required for Wg release from the producing
cells, its spreading or its transduction? The answer is
unclear. On one hand, the shits embryonic phenotype is
reminiscent of a secretion-defective Wg mutant,
suggesting that endocytic block affects Wg release
(Bejsovec and Wieschaus, 1995; Gonzalez et al., 1991).
This possibility has also been proposed for Wg during
wing development (Strigini and Cohen, 1999). On the
other hand, endocytic block restricted to the receiving
cells also affects Wg signaling, consistent with a
endocytic role during either spreading or transduction of
the signal (Moline et al., 1999).
Like in the case of Dpp, a possible role of endocytosis
during the spreading of Wg is that it initiates the planar
transcytosis of the morphogen: Wg is internalized by
endocytosis, traffics through the endocytic pathway and is
re-secreted again to move further into the target tissue.
Wg recycling in this way was observed using a functional
Wg-GFP fusion (Pfeiffer et al., 2002). Fluorescence time-
lapse microscopy of Wg-GFP shows that the Wg
internalized in endocytic vesicles can return to the cell
surface. Although recycling could only be observed in the
apical surface, which is optically accessible, it is still
possible that re-secretion also occurs laterally within the
epithelium, thereby directing the ligand to the neighbour-
ing cells. Ligand recycling is a key feature of the planar
transcytosis model of transport: the ligand spreads by
repeated cycles of internalization, recycling, and presen-
tation to further cells. The observation of Wingless
recycling shows that planar transcytosis is plausible.
However, one should note that, in the above experimental
situation, very few endocytic vesicles containing GFP-
Wingless were present in non-expressing cells. Therefore,
either a small number of vesicles are sufficient for
transport or transcytosis is not an important contributor
to Wg transport.
In the wing, it has been argued that endocytosis is indeed
not required for the dispersal of the signal. This was based
on the absence of Wg shadows (Strigini and Cohen, 1999)
when performing a shadow assay as described above for
Dpp (Entchev et al., 2000). However, in the case of the Wg
experiment, the shadow assay was performed in a steady-
state situation. In this experimental condition, before Wg
disappears from the distal side of the endocytosis-defective
mutant clone, molecules of Wg emanating from the sides
will fill this distal region rapidly. As a consequence, like in
the case of Dpp, no distal Wg shadows will be formed if the
experiment is started in a steady-state situation if Wg moves
rapidly and in all directions. Wg moves rapidly: the gradient
can expand at a speed of 15 cells in 30 min. It also moves in
all directions. To observe shadows the experiment should be
done in conditions in which the propagation front of Wg
gradient expansion meets a clone of Shibire mutant cells as
performed in the Dpp shadow assay.
M. Gonzalez-Gaitan / Mechanisms of Development 120 (2003) 1265–12821274
Whatever the mechanism of Wg dispersal (diffusion vs.
planar transcytosis), is Wg transported in vesicular struc-
tures while spreading through the receiving tissue? A recent
report shows that, like Hh (see below), Wingless is
palmitoylated (Willert et al., 2003), suggesting that it
would not appear as a soluble protein in the extracellular
space, but associated to a lipidic millieu. Interestingly, Wg
has been seen in the same endocytic compartment as the
argosomes, lipidic fragments that disperse over long
distances in the wing epithelium (Greco et al., 2001). The
molecular and cellular nature of the argosomes and the
question whether they serve as lipidic carriers for signaling
molecules such as Wg or Hh remains yet to be fully
understood, but such mechanism of morphogen dispersal is
certainly tantalizing.
3. Trafficking during short-range morphogenetic
signaling: Hh in the wing and the embryo
Like Dpp and Wg, Hh forms concentration gradients
during development which instructs cells about their
positional information. Hh shows post-tranlational modifi-
cations by covalent binding to two lipid moieties:
cholesterol (Porter et al., 1996) and palmitoyl acid
(Chamoun et al., 2001; Pepinsky et al., 1998). This implies
that Hh is a membrane-tethered molecule. Indeed Hh range
of spreading is shorter than for other morphogens, such as
Dpp. In the case of the developing wing Hh elicits signaling
not farther beyond 10 cells and in the embryo, not beyond
four cells. But being membrane-tethered, how is Hh
released from the producing cells? How does it spread
through the target tissues? What are the mechanisms
underlying the transduction of the signal? These are indeed
unsolved issues.
In the producing cells, Hh family proteins undergo a
autoproteolytic cleavage under the control of the C-terminal
domains. Concomitantly, a cholesterol moiety is added to
Hh N-terminal domain at its C-terminus to give raise to the
active Hh fragment, which is thereby linked to the
membrane (Beachy et al., 1997) and is found in lipid rafts
(Rietveld et al., 1999). Strikingly, the cholesterol-modified
membrane-tethered N-terminal Hh fragment carries the
morphogenetic signaling functions both at long- and short-
range, while the C-terminal domain, secreted and soluble, is
inactive for signaling (Beachy et al., 1997). Another lipid
modification of Hh, a palmitoylation of its N-terminal
cysteine, has been shown to occur in vertebrates and
Drosophila (Chamoun et al., 2001; Pepinsky et al., 1998).
The factor that catalyses Hh palmitoylation, Skinny hedge-
hog, shares sequence homology with O-linked acyl
transferases. These are cytosolic enzymes that therefore
add the palmitoyl moiety to the cytoplasmic side of
transmembrane proteins. It is therefore intriguing how, in
the case of Hh, they catalyse the lipid modification on the
luminal side of the protein.
3.1. Hh release and spreading: cholesterol modification
What are these lipid modifications good for? In the case
of the cholesterol modification, it is controversial whether
cholesterol modification restricts or widens the range of
secreted Hh. This question was addressed using a truncated
N-terminal Hedgehog transgene which does not undergo
cholesterol modification (Burke et al., 1999; Lewis et al.,
2001). In a mesenchymal situation, the developing mouse
limb, this non-modified Hh is only able to elicit short-range
signaling, suggesting that the cholesterol modification is
essential for long-range spreading of the ligand (Lewis et al.,
2001). In contrast, in an epithelial situation, the Drosophila
developing wing, the corresponding non-modified Hh
shows a longer spreading range, leading to the opposite
proposal that the cholesterol moiety restricts Hh spreading.
In the case of the wing, absence of cholesterol modification
leads to a mistargeting of Hh release (Burke and Basler,
1996): in the wildtype, Hh is seen in the basolateral side of
the epithelium, while non-cholesterol-modified Hh is found
in the apical side of the developing wing. This raises the
possibility that cholesterol controls Hh secretion into a side
of the epithelium where the extracellular milieu might
determine the range of spreading. Thus, while the apical,
luminal side of the developing wing will allow free-
diffusion of Hh to a long distance from the source, in the
case of the mesenchymal cells, the limiting factor might not
be release/spreading, but the transduction of the signal (see
below). In another developing context, the embryonic
segmentation of the epidermis, the cholesterol modification
of Hh has also been recently shown to be responsible for its
targeting to large punctate structures, possibly an endocytic
compartment, at the apical pole of the receiving cells (Gallet
et al., 2003). The proper targeting of cholesterol-modified
Hh is mediated by a sterol-sensing domain protein,
Dispatched (Burke et al., 1999; Ma et al., 2002). It is
therefore possible that cholesterol modification endows Hh
with targeting information during trafficking in polarized
epithelial cells, a role for cholesterol which is reminiscent of
cholesterol-enriched lipid rafts in apical targeting in the
biosynthetic pathway of epithelial cells (Simons and Ikonen,
1997). Once properly targeted to the right side of the cells,
Hh is released to a extracellular space of the epithelium
where proteoglycans synthesized by the GAG transferase
enzyme Tout-velou mediate the movement of modified Hh
throughout the tissue (Bellaiche et al., 1998; Gallet et al.,
2003; The et al., 1999).
In addition to the role of cholesterol modification and
proteoglycans, the Hh receptor Patched (Ptc) also plays a
key role to restrict Hh spreading. High levels of Ptc restricts
Hh movement throughout the tissue (Chen and Struhl,
1996): Ptc overexpressing clones cast shadows behind, like
in the shadow assay. Hh is involved this way in an
autoregulatory loop that limits its spreading: Hh signaling
upregulates Ptc, which in turn binds to Hh and titrates it,
impeding its long-range movement. Subsequently, the levels
M. Gonzalez-Gaitan / Mechanisms of Development 120 (2003) 1265–1282 1275
of Ptc at the plasma membrane are regulated by Dynamin-
dependent internalization initiated by Ptc binding to Hh
(Denef et al., 2000), which lead to targeting to endocytic
vesicles and MVBs (Capdevila et al., 1994). It is, however,
unclear whether endocytosis itself plays any role during Hh
spreading and to date no data suggests that Hh movement
involves a planar transcytosis mechanism.
3.2. Hh signal transduction and the endocytic pathway
Ptc acts as a Hh receptor, but instead of eliciting signaling,
its function is to repress the signaling pathway. In the absence
of the ligand, Ptc inhibits a latent, tonic signaling activity of
another transmembrane protein, Smoothened (Smo)
(reviewed in Ingham and McMahon, 2001). Ptc binding
destabilizes Smo (Denef et al., 2000). Binding of Hh to Ptc,
releases its inhibition of Smo. This release is mediated by
Hh-induced internalization of Ptc, followed by phosphoryl-
ation of Smo, which in turn is stabilized and accumulates at
the plasma membrane (Denef et al., 2000). These obser-
vations suggested that Hh elicits signaling by diverting Ptc
into a distinct trafficking route that would release Smo from
Ptc repression. Consistent with this, a mutant in the sterol-
sensing domain of Ptc which is not affected in binding/
sequestration of Hh, is unable to repress the intrinsic
signaling activity of Smo (Chen and Struhl, 1996; Martin
et al., 2001; Strutt et al., 2001). The sterol-sensing domain
has been implicated in the targeting of proteins and lipids
through specific membrane compartments (Kuwabara and
Labouesse, 2002). Indeed, the sterol-sensing domain mutants
in Ptc are mistargeteds and do not anymore colocalize with
Smo in the endocytic compartment (Martin et al., 2001). In
summary, the role of Hh as a signaling molecule would then
be to get rid of a molecule, Ptc, that acts as a repressor of a
Smo-dependent tonic signaling.
In mammalian cells in culture, the intricacies of this
fascinating possibility have been studied in some detail by
the Roelink group (Incardona et al., 2002). Ptc and Smo
colocalize extensively in the absence of Sonic Hedgehog
(Shh), a mammalian Hh homolog. Upon ligand binding,
Shh, Ptc and Smo are internalized together, but become
subsequently segregated into different compartments: the
Ptc-Hh complex is targeted for degradation at the lysosome
while Smo is not. The sorting of Smo requires an acid
luminal endosomal environment in which the membrane is
enriched in lysobiphosphatidic acid (LBPA), suggesting a
specific trafficking pathway during Hh signaling.
3.3. Cholesterol-dependent Hh trafficking and Hh
functional diversity
Cholesterol modification of Hh and the sterol-sensing
domain in Ptc may play key roles in trafficking through this
specific pathway. An interesting possibility is that, during
Hh signaling, activation of different target genes is mediated
by Hh presentation from different membrane compartments
determined by the lipid modification of Hh (Gallet et al.,
2003). This has been suggested for Hh signaling during
epidermal embryonic segmentation (Fig. 5). As described
above, Hh is expressed in two rows of cells abutting the
parasegmental boundary in the embryonic epidermis and
from there (i) activates Wg in the cells adjacent in the
anterior direction and (ii) activates Rho in three cell rows
towards the posterior direction (Fig. 5A,B). Targeting of Hh
to an apical compartment in the receiving cells (Fig. 5A,C)
depends on cholesterol modification and the function of the
sterol-sensing domain protein Dispatched (disp), which has
being implicated previously in Hh release from the
producing cells (Burke et al., 1999; Ma et al., 2002). In
non-cholesterol-modified hh or in disp mutants, apical
targeting of Hh in the receiving cells is absent. These mutant
conditions abolish Hh signaling in the anterior adjacent
cells, but do not affect signaling towards the posterior cells,
which thereby activate Rho normally (Gallet et al., 2003).
Similarly, Tout-velu mutants affect anterior Wg expression,
but not posterior signaling. Tout-velu promotes the spread-
ing of cholesterol-modified Hh through the extracellular
space by catalyzing the synthesis of a proteoglycan that
mediates Hh movement.
In summary, anterior signaling requires Hh targeting to
the apical endosome to be properly released from the
producing cells in a process which requires Cholesterol
modification of Hh, its release in Disp-dependent manner
and the proteoglycan-dependent spreading of cholesterol-
modified Hh mediated by Tout-velu (Fig. 5C). In contrast,
posterior signaling does not require Hh modification with
cholesterol, its release or proteoglycan-mediated movement
(Fig. 5C). This uncovers a scenario in which different
cellular environments are able to elicit the expression of
different target genes depending on the lipid modification
and thereby the subcellular compartment (i.e. the apical
endosomal compartment where Hh is normally found) in
which the Hh ligand is present.
It is, however, unclear how a Hh molecule which has not
been cholesterol-modified, that cannot be released properly
(in disp mutants) or cannot spread through a long-range (in
Tout-velu mutants) is nevertheless able to elicit signaling
across 3–4 cell diameters in the posterior direction.
Conversely, it is surprising that all these cellular require-
ments, which are essential for long-range spreading of
the ligand, are essential to signal to the neighbour anterior
cell. These paradoxes reflect that probably we are missing
some essential cellular/molecular process at the basis of
asymmetric Hh signaling during the process of
segmentation.
4. Endocytic trafficking during lateral inhibition: Notch
signaling and asymmetric cell division
Dpp, Hh and Wg form gradients of concentration that
elicits signaling in cells at a distance from the source.
M. Gonzalez-Gaitan / Mechanisms of Development 120 (2003) 1265–12821276
During asymmetric cell division (ACD), the Notch signal-
ing pathway mediates lateral inhibition between two
adjacent cells contacting each other. Asymmetric Notch
signaling probably capitalizes on asymmetric endocytic
trafficking.
4.1. Asymmetric localization of Numb controls Notch
signaling during ACD
The external sense organs (ES) of the PNS are
composed of two outer cells (hair and socket), two inner
cells (neuron and sheath) and a glial cell (Fig. 6A) (Gho
et al., 1999). These four cells arise from a single sensory
organ precursor (SOP) cell in a stereotyped lineage:
the SOP divides into a posterior pIIa and an anterior pIIb
cell; pIIb generates the pIIIb and a glial cell, pIIa the hair
and the socket and pIIIb the neuron and the sheath
(Fig. 6B) (Gho et al., 1999).
Numb, a phosphotyrosine binding protein, determines
the fate of the SOP progeny (Rhyu et al., 1994; Uemura
et al., 1989): in loss of function numb mutants SOPs divide
symmetrically into two pIIa cells, which subsequently
generate two sockets (Fig. 6C). Conversely, Numb over-
expression in the SOP lead to the generation of four neurons.
Fig. 5. Cholesterol and asymmetric Hh signaling? (A,B) Hh signaling (blue) activates Wg (red) in the anterior adjacent cells and Rho (green) within a range of 3
cell diameters towards the posterior. In receiving cells, Hh is internalized into ‘large punctate structures’ (LPS) probably corresponding to an apical endosomal
structure. (A) Z section through the epithelium. (B) XY section. (C) Hh is secreted from the source (blue nucleus) by a process that requires Disp. It is
internalized into an LPS in a process that requires Ttv. Anterior signaling to activate Wg (red) requires Disp, Ttv and the cholesterol moiety (Hh-Np). Posterior
signaling to activate Rho (green) is independent of Hh release, Disp, Ttv and the cholesterol moiety.
M. Gonzalez-Gaitan / Mechanisms of Development 120 (2003) 1265–1282 1277
Fig. 6. Endocytosis and asymmetric cell division. (A) Schematic representation of an ES organ. (B) Schematic representation of the asymmetric cell divisions
that give rise to the five cells in the ES organ. (C,D) numb2/a-adaptinear (C) and Nts (D) mutant phenotypes. (E) Molecular interactions between Notch, Numb,
a-adaptin and Clathrin. (F) Notch binding of Numb recruits a-adaptin/Clathrin thereby initiating its internalization by endocytosis. (G) A model for the role of
endocytosis during asymmetric cell division. Numb distributed in a crescent in the SOP causes the asymmetric distribution of a-adaptin. Higher levels of
Numb/a-adaptin in one cell causes the enhanced down-regulation of Notch by endocytosis in that cell. This gives advantage to one of the two cells during
mutual competition for Delta/Notch signaling. This initial bias is increased until it is converted into a directional Notch signaling from one of the two cells, that
inhibits the PIIa fate in the adjacent cell.
M. Gonzalez-Gaitan / Mechanisms of Development 120 (2003) 1265–12821278
Interestingly, in the SOPs, the Numb protein concentrates in
the area of the cortex that overlies one of the two
centrosomes (Knoblich et al., 1995) and is segregated into
one of the two daughter cells upon cytokinesis (Fig. 6G)
(Rhyu et al., 1994). Therefore, Numb behaves as a
segregating determinant in the SOP lineage.
Numb controls ACD by repressing Notch signaling.
Notch is the receptor of two ligands, Delta and Serrate,
which upon binding lead to Notch cleavage. The intracellu-
lar Notch fragment is then imported into the nucleus and
converts Suppressor of Hairless, a repressor, into a
transcriptional activator. Inactivation of Notch function
during ACD lead to cell fate transformations which are the
opposite to those observed in numb mutants: SOP divides
into two pIIb which generate four neurons (Fig. 6D)
(Hartenstein and Posakony, 1989). Numb acts upstream of
Notch (Guo et al., 1996) and both molecules bind to each
other (Guo et al., 1996). A model has been suggested (Zeng
et al., 1998) in which both Delta and Serrate bind to Notch
in the SOP lineage: Notch signaling induces pIIa fate in one
daughter cell, while Numb prevents Notch signal transduc-
tion in the other, which thereby adopts the pIIb fate.
How does Numb control Notch signal transduction? A
mammalian Numb homolog localizes to endocytic vesicles
and binds to a-Adaptin, a component of the AP2 complex
(Santolini et al., 2000). AP2 initiates Clathrin coating in
endocytic vesicles by recruiting Clathrin to the endocytic
bud and triggering Clathrin polymerization into a lattice.
That prompted the possibility that Numb controls Notch
signaling by orchestrating the endocytosis of the receptor. It
was already known that Dynamin plays a key role during
Notch signaling (Seugnet et al., 1997).
4.2. Endocytosis, Notch signaling and ACD
Another endocytic factor, a-Adaptin, plays a specific
role during ACD. a-Adaptin mutants were recovered in a
screen for factors involved in ACD (Berdnik et al., 2002).
a-Adaptin is composed of a head domain, an ear domain
and a hinge domain. While loss of function mutations in
a-Adaptin blocks endocytosis and cause embryonic leth-
ality (Gonzalez-Gaitan and Jackle, 1997), mutations in the
ear domain of a-Adaptin cause a milder phenotype and
resemble Numb loss of function mutations during ES
development (Fig. 6C). The ear domain of a-Adaptin has a
regulatory role during endocytosis by binding to accessory
endocytic proteins including AP-180, Epsin, EPS-15,
Dynamin and Amphiphysin. It was also shown to bind to
mammalian Numb (Santolini et al., 2000). Furthermore, it
was shown that the ear domain of Drosophila a-Adaptin is
able to bind Numb both in vitro and in vivo (Berdnik et al.,
2002). The Numb binding domain contains a DPF domain
that was shown to be essential for Notch repression (Frise
et al., 1996).
In the asymmetrically dividing SOPs, a-Adaptin, like
Numb, is concentrated to one side of the cell cortex
during metaphase (Fig. 6G) (Berdnik et al., 2002). During
cell fate specification in the Drosophila ES lineage, a-
Adaptin acts downstream of Numb and upstream of
Notch: in numb mutants a-Adaptin fails to localize
asymmetrically. Since Numb can directly interact with
Notch intracellular domain, Numb may antagonize Notch
activity by recruiting a-Adaptin (Fig. 6E). This would in
turn initiate Notch internalization by Clathrin-mediated
endocytosis (Fig. 6F) and ultimately cause down-regu-
lation of Notch signaling in the cells that get the higher
levels of Numb/a-Adaptin (Fig. 6G). Testing this
hypothesis will require Notch internalization assays in
vivo during the development of ES.
5. Concluding remarks
Different signaling events capitalize on endocytic
trafficking in different ways: endocytic trafficking powers
the long-range spreading of Dpp, but is also used to restrict
the range of Wg signaling in the embryo; it is used to
implement Hh signaling by degrading the repressing
receptor, Ptc and trafficking it away from the tonic activator
Smo and, during Notch signaling in ACD, to have a biased
internalization of the receptor, thereby skewing a reciprocal
signaling event. These proposed models of action for
endocytosis are qualitative, while their basis is the
quantitative change in the rates of internalization, degra-
dation and recycling. To fully understand the mechanisms,
we will need to examine these processes in quantitative
detail. Therefore, future directions will include the
quantitative assessment of the rates of trafficking and
signaling.
In Drosophila, tools like the thermosensitive shibire
mutant have provided the possibility of studying phenotypes
in real time, a key tool when monitoring trafficking. The
analysis of other kinds of mutants only allows monitoring of
the effects of the mutations after the developing system
reaches its steady-state. This means that many of these
phenotypes could be indirect, the consequence of the reaction
of a system which probably has backups built in. In the future,
a useful tool to help us understand the trafficking mechanisms
during signaling would be conditional mutant situations that
allow us to study the direct cell biological effects of depleting
a gene function in real time.
Acknowledgements
I would like to thank Karen Echeverri, Christian Bokel
and Alfonso Martınez-Arias for critically reading this
manuscript. My work is supported by the Max-Planck
Society and DFG.
M. Gonzalez-Gaitan / Mechanisms of Development 120 (2003) 1265–1282 1279
References
Alexandre, C., Lecourtois, M., Vincent, J., 1999. Wingless and Hedgehog
pattern Drosophila denticle belts by regulating the production of short-
range signals. Development 126, 5689–5698.
Banerjee, U., Renfranz, P.J., Hinton, D.R., Rabin, B.A., Benzer, S., 1987.
The sevenless þ protein is expressed apically in cell membranes of
developing Drosophila retina; it is not restricted to cell R7. Cell 51,
151–158.
Beachy, P.A., Cooper, M.K., Young, K.E., von Kessler, D.P., Park, W.J.,
Hall, T.M., et al., 1997. Multiple roles of cholesterol in hedgehog
protein biogenesis and signaling. Cold Spring Harb Symp Quant Biol
62, 191–204.
Bejsovec, A., Wieschaus, E., 1995. Signaling activities of the Drosophila
wingless gene are separately mutable and appear to be transduced at the
cell surface. Genetics 139, 309–320.
Bellaiche, Y., The, I., Perrimon, N., 1998. Tout-velu is a Drosophila
homologue of the putative tumour suppressor EXT-1 and is needed for
Hh diffusion. Nature 394, 85–88.
Bennett, D., Alphey, L., 2002. PP1 binds Sara and negatively regulates Dpp
signaling in Drosophila melanogaster. Nat. Genet. 31, 419–423.
Berdnik, D., Torok, T., Gonzalez-Gaitan, M., Knoblich, J.A., 2002. The
endocytic protein alpha-Adaptin is required for numb-mediated
asymmetric cell division in Drosophila. Dev. Cell 3, 221–231.
Burke, R., Basler, K., 1996. Dpp receptors are autonomously required for
cell proliferation in the entire developing wing. Development 122,
2261–2269.
Burke, R., Nellen, D., Bellotto, M., Hafen, E., Senti, K.A., Dickson, B.J.,
Basler, K., 1999. Dispatched, a novel sterol-sensing domain protein
dedicated to the release of cholesterol-modified hedgehog from
signaling cells. Cell 99, 803–815.
Capdevila, J., Pariente, F., Sampedro, J., Alonso, J.L., Guerrero, I., 1994.
Subcellular localization of the segment polarity protein patched
suggests an interaction with the wingless receptor complex in
Drosophila embryos. Development 120, 987–998.
Chamoun, Z., Mann, R.K., Nellen, D., von Kessler, D.P., Bellotto, M.,
Beachy, P.A., Basler, K., 2001. Skinny hedgehog, an acyltransferase
required for palmitoylation and activity of the hedgehog signal. Science
293, 2080–2084.
Chen, Y., Struhl, G., 1996. Dual roles for Patched in sequestering and
transducing Hedgehog. Cell 87, 553–563.
Denef, N., Neubueser, D., Perez, L., Cohen, S.M., 2000. Hedgehog induces
opposite changes in turnover and subcellular localization of patched and
smoothened. Cell 102, 521–531.
Di Guglielmo, G.M., Le Roy, C., Goodfellow, A.F., Wrana, J.L., 2003.
Distinct endocytic pathways regulate TGF-beta receptor signalling and
turnover. Nat. Cell Biol. 5, 410–421.
DiNardo, S., Sher, E., Heemskerk-Jongens, J., Kassis, J.A., O’Farrell, P.H.,
1988. Two-tiered regulation of spatially patterned engrailed gene
expression during Drosophila embryogenesis. Nature 332, 604–609.
Dubois, L., Lecourtois, M., Alexandre, C., Hirst, E., Vincent, J.P., 2001.
Regulated endocytic routing modulates wingless signaling in Droso-
phila embryos. Cell 105, 613–624.
Ebisawa, T., Fukuchi, M., Murakami, G., Chiba, T., Tanaka, K., Imamura,
T., Miyazono, K., 2001. Smurf1 interacts with transforming growth
factor-beta type I receptor through Smad7 and induces receptor
degradation. J. Biol. Chem. 276, 12477–12480.
Entchev, E.V., Schwabedissen, A., Gonzalez-Gaitan, M., 2000. Gradient
formation of the TGF-beta homolog Dpp. Cell 103, 981–991.
Fehon, R.G., Johansen, K., Rebay, I., Artavanis-Tsakonas, S., 1991.
Complex cellular and subcellular regulation of notch expression during
embryonic and imaginal development of Drosophila: implications for
notch function. J. Cell Biol. 113, 657–669.
Frise, E., Knoblich, J.A., Younger-Shepherd, S., Jan, L.Y., Jan, Y.N., 1996.
The Drosophila Numb protein inhibits signaling of the Notch receptor
during cell–cell interaction in sensory organ lineage. Proc. Natl Acad.
Sci. USA 93, 11925–11932.
Gallet, A., Rodriguez, R., Ruel, L., Therond, P.P., 2003. Cholesterol
modification of hedgehog is required for trafficking and movement,
revealing an asymmetric cellular response to hedgehog. Dev. Cell 4,
191–204.
Gho, M., Bellaiche, Y., Schweisguth, F., 1999. Revisiting the Drosophila
microchaete lineage: a novel intrinsically asymmetric cell division
generates a glial cell. Development 126, 3573–3584.
Gillooly, D.J., Morrow, I.C., Lindsay, M., Gould, R., Bryant, N.J., Gaullier,
J.M., Parton, R.G., Stenmark, H., 2000. Localization of phosphatidyl-
inositol 3-phosphate in yeast and mammalian cells. Eur. Mol. Biol. Org.
J. 19, 4577–4588.
Gillooly, D.J., Simonsen, A., Stenmark, H., 2001. Cellular functions of
phosphatidylinositol 3-phosphate and FYVE domain proteins. Bio-
chem. J. 355, 249–258.
Golembo, M., Raz, E., Shilo, B.Z., 1996. The Drosophila embryonic
midline is the site of Spitz processing, and induces activation of the
EGF receptor in the ventral ectoderm. Development 122, 3363–3370.
Gonzalez, F., Swales, L.S., Bejsovec, A., Skaer, H., Martinez Arias, A.,
1991. Secretion and movement of wingless protein in the epidermis of
the Drosophila embryo. Mech. Dev. 35, 43–54.
Gonzalez-Gaitan, M.A., Jackle, H., 1997. Role of Drosophila a-adaptin
during synaptic vesicle recycling. Cell 88, 767–776.
Gonzalez-Gaitan, M.A., Jackle, H., 1999. The range of spalt-activating Dpp
signalling is reduced in endocytosis-defective Drosophila wing discs.
Mech. Dev. 87, 143–151.
Greco, V., Hannus, M., Eaton, S., 2001. Argosomes: a potential vehicle for
the spread of morphogens through epithelia. Cell 106, 633–645.
Grindstaff, K.K., Yeaman, C., Anandasabapathy, N., Hsu, S.C., Rodriguez-
Boulan, E., Scheller, R.H., Nelson, W.J., 1998. Sec6/8 complex is
recruited to cell–cell contacts and specifies transport vesicle delivery to
the basal–lateral membrane in epithelial cells. Cell 93, 731–740.
Gritzan, U., Hatini, V., DiNardo, S., 1999. Mutual antagonism between
signals secreted by adjacent wingless and engrailed cells leads to
specification of complementary regions of the Drosophila parasegment.
Development 126, 4107–4115.
Guo, M., Jan, L.Y., Jan, Y.N., 1996. Control of daughter cell fates during
asymmetric division: interaction of Numb and Notch. Neuron 17,
27–41.
Hartenstein, V., Posakony, J.W., 1989. Development of adult sensilla on the
wing and notum of Drosophila melanogaster. Development 107,
389–405.
Hayes, S., Chawla, A., Corvera, S., 2002. TGF beta receptor internalization
into EEA1-enriched early endosomes: role in signaling to Smad2. J. Cell
Biol. 158, 1239–1249.
van den Heuvel, M., Nusse, R., Johnston, P., Lawrence, P.A., 1989.
Distribution of the wingless gene product in Drosophila embryos: a
protein involved in cell–cell communication. Cell 59, 739–749.
Incardona, J.P., Gruenberg, J., Roelink, H., 2002. Sonic hedgehog induces
the segregation of patched and smoothened in endosomes. Curr. Biol.
12, 983–995.
Ingham, P.W., McMahon, A.P., 2001. Hedgehog signaling in animal
development: paradigms and principles. Genes Dev. 15, 3059–3087.
Ingham, P.W., Baker, N.E., Martinez-Arias, A., 1988. Regulation of
segment polarity genes in the Drosophila blastoderm by fushi tarazu
and even skipped. Nature 331, 73–75.
Itoh, F., Divecha, N., Brocks, L., Oomen, L., Janssen, H., Calafat, J., et al.,
2002. The FYVE domain in Smad anchor for receptor activation
(SARA) is sufficient for localization of SARA in early endosomes and
regulates TGF-beta/Smad signalling. Genes Cells 7, 321–331.
Iwasaki, S., Tsuruoka, N., Hattori, A., Sato, M., Tsujimoto, M., Kohno, M.,
1995. Distribution and characterization of specific cellular binding
proteins for bone morphogenetic protein-2. J. Biol. Chem. 270,
5476–5482.
Kavsak, P., Rasmussen, R.K., Causing, C.G., Bonni, S., Zhu, H., Thomsen,
G.H., Wrana, J.L., 2000. Smad7 binds to Smurf2 to form an E3
M. Gonzalez-Gaitan / Mechanisms of Development 120 (2003) 1265–12821280
ubiquitin ligase that targets the TGF beta receptor for degradation. Mol.
Cell 6, 1365–1375.
Knoblich, J.A., Jan, L.Y., Jan, Y.N., 1995. Asymmetric segregation of
Numb and Prospero during cell division. Nature 377, 624–627.
Kuwabara, P.E., Labouesse, M., 2002. The sterol-sensing domain: multiple
families, a unique role? Trends Genet. 18, 193–201.
Lander, A.D., Nie, Q., Wan, F.Y., 2002. Do morphogen gradients arise by
diffusion? Dev. Cell 2, 785–796.
Lanzetti, L., Rybin, V., Malabarba, M.G., Christoforidis, S., Scita, G.,
Zerial, M., Di Fiore, P.P., 2000. The Eps8 protein coordinates EGF
receptor signalling through Rac and trafficking through Rab5. Nature
408, 374–377.
Lauffenburger, D.A., Linderman, J.J., 1993. Receptors. Models for
Binding, Trafficking and Signaling, Oxford University Press, New
York.
Lecuit, T., Cohen, S.M., 1998. Dpp receptor levels contribute to shaping the
Dpp morphogen gradient in the Drosophila wing imaginal disc.
Development 125, 4901–4907.
Lecuit, T., Brook, W.J., Ng, M., Calleja, M., Sun, H., Cohen, S.M., 1996.
Two distinct mechanisms for long-range patterning by decapentaplegic
in the Drosophila wing. Nature 381, 387–393.
Lewis, P.M., Dunn, M.P., McMahon, J.A., Logan, M., Martin, J.F., St-
Jacques, B., McMahon, A.P., 2001. Cholesterol modification of sonic
hedgehog is required for long-range signaling activity and effective
modulation of signaling by Ptc1. Cell 105, 599–612.
Lin, X., Liang, M., Feng, X.H., 2000. Smurf2 is a ubiquitin E3 ligase
mediating proteasome-dependent degradation of Smad2 in transform-
ing growth factor-beta signaling. J. Biol. Chem. 275, 36818–36822.
Ma, Y., Erkner, A., Gong, R., Yao, S., Taipale, J., Basler, K., Beachy, P.A.,
2002. Hedgehog-mediated patterning of the mammalian embryo
requires transporter-like function of dispatched. Cell 111, 63–75.
Martin, V., Carrillo, G., Torroja, C., Guerrero, I., 2001. The sterol-sensing
domain of Patched protein seems to control Smoothened activity
through Patched vesicular trafficking. Curr. Biol. 11, 601–607.
Martinez Arias, A., 2003. Wnts as morphogens? The view from the wing of
Drosophila. Nat. Rev. Mol. Cell Biol. 4, 321–325.
Massague, J., 1998. TGF-b signal transduction. Annu. Rev. Biochem. 67,
753–791.
Massague, J., Kelly, B., 1986. Internalization of transforming growth
factor-beta and its receptor in BALB/c 3T3 fibroblasts. J. Cell Physiol.
128, 216–222.
Miyazono, K., 2000. TGF-beta signaling by Smad proteins. Cytokine
Growth Factor Rev. 11, 15–22.
Moline, M.M., Southern, C., Bejsovec, A., 1999. Directionality of Wingless
protein transport influences epidermal patterning in the Drosophila
embryo. Development 126, 4375–4384.
Mukherjee, S., Ghosh, R.N., Maxfield, F.R., 1997. Endocytosis. Physiol.
Rev. 77, 759–803.
Natsume, T., Tomita, S., Iemura, S., Kinto, N., Yamaguchi, A., Ueno, N.,
1997. Interaction between soluble type I receptor for bone morpho-
genetic protein and bone morphogenetic protein-4. J. Biol. Chem. 272,
11535–11540.
Nellen, N., Burke, R., Struhl, G., Basler, K., 1996. Direct and long-range
action of a DPP morphogen gradient. Cell 85, 357–368.
Novick, P., Zerial, M., 1997. The diversity of Rab proteins in vesicle
transport. Curr. Opin. Cell Biol. 9, 496–504.
Panopoulou, E., Gillooly, D.J., Wrana, J.L., Zerial, M., Stenmark, H.,
Murphy, C., Fotsis, T., 2002. Early endosomal regulation of Smad-
dependent signaling in endothelial cells. J. Biol. Chem. 277,
18046–18052.
Payre, F., Vincent, A., Carreno, S., 1999. ovo/svb integrates Wingless and
DER pathways to control epidermis differentiation. Nature 400,
271–275.
Penheiter, S.G., Mitchell, H., Garamszegi, N., Edens, M., Dore, J.J. Jr.,
Leof, E.B., 2002. Internalization-dependent and -independent require-
ments for transforming growth factor beta receptor signaling via the
Smad pathway. Mol. Cell Biol. 22, 4750–4759.
Pepinsky, R.B., Zeng, C., Wen, D., Rayhorn, P., Baker, D.P., Williams,
K.P., et al., 1998. Identification of a palmitic acid-modified form of
human Sonic hedgehog. J. Biol. Chem. 273, 14037–14045.
Pfeiffer, S., Ricardo, S., Manneville, J.B., Alexandre, C., Vincent, J.P.,
2002. Producing cells retain and recycle Wingless in Drosophila
embryos. Curr. Biol. 12, 957–962.
Podos, S.D., Hanson, K.K., Wang, Y.C., Ferguson, E.L., 2001. The DSmurf
ubiquitin-protein ligase restricts BMP signaling spatially and tem-
porally during Drosophila embryogenesis. Dev. Cell 1, 567–578.
Porter, J.A., Young, K.E., Beachy, P.A., 1996. Cholesterol modification of
Hedgehog signaling proteins in animal development. Science 274,
255–259.
Rhyu, M.S., Jan, L.Y., Jan, Y.N., 1994. Asymmetric distribution of numb
protein during division of the sensory organ precursor cell confers
distinct fates to daughter cells. Cell 76, 477–491.
Rietveld, A., Neutz, S., Simons, K., Eaton, S., 1999. Association of sterol-
and glycosylphosphatidylinositol-linked proteins with Drosophila raft
Lipid microdomains. J. Biol. Chem. 274, 12049–12054.
Sanson, B., Alexandre, C., Fascetti, N., Vincent, J.P., 1999. Engrailed and
hedgehog make the range of Wingless asymmetric in Drosophila
embryos. Cell 98, 207–216.
Santolini, E., Puri, C., Salcini, A.E., Gagliani, M.C., Pelicci, P.G.,
Tacchetti, C., Di Fiore, P.P., 2000. Numb is an endocytic protein.
J. Cell Biol. 151, 1345–1352.
Sathre, K.A., Tsang, M.L., Weatherbee, J.A., Steer, C.J., 1991. Binding and
internalization of transforming growth factor-beta 1 by human
hepatoma cells: evidence for receptor recycling. Hepatology 14,
287–295.
Seugnet, L., Simpson, P., Haenlin, M., 1997. Requirement for dynamin
during Notch signaling in Drosophila neurogenesis. Dev. Biol. 192,
585–598.
Sheff, D.R., Daro, E.A., Hull, M., Mellman, I., 1999. The receptor recycling
pathway contains two distinct populations of early endosomes with
different sorting functions. J. Cell Biol. 145, 123–139.
Shitara, Y., Kato, Y., Sugiyama, Y., 1998. Effect of brefeldin A and
lysosomotropic reagents on intracellular trafficking of epidermal
growth factor and transferrin in Madin–Darby canine kidney epithelial
cells. J. Control Release 55, 35–43.
Simons, K., Ikonen, E., 1997. Functional rafts in cell membranes. Nature
387, 569–572.
Strigini, M., Cohen, S.M., 1999. Formation of morphogen gradients in the
Drosophila wing. Semin. Cell Dev. Biol. 10, 335–344.
Strutt, H., Thomas, C., Nakano, Y., Stark, D., Neave, B., Taylor, A.M.,
Ingham, P.W., 2001. Mutations in the sterol-sensing domain of Patched
suggest a role for vesicular trafficking in Smoothened regulation. Curr.
Biol. 11, 608–613.
Tall, G.G., Barbieri, M.A., Stahl, P.D., Horazdovsky, B.F., 2001. Ras-
activated endocytosis is mediated by the Rab5 guanine nucleotide
exchange activity of RIN1. Dev. Cell 1, 73–82.
The, I., Bellaiche, Y., Perrimon, N., 1999. Hedgehog movement is
regulated through Tout velu-dependent synthesis of a heparan sulfate
proteoglycan. Mol. Cell 4, 633–639.
Tomlinson, A., Bowtell, D.D., Hafen, E., Rubin, G.M., 1987. Localization
of the sevenless protein, a putative receptor for positional information,
in the eye imaginal disc of Drosophila. Cell 51, 143–150.
Tsukazaki, T., Chiang, T.A., Davidson, A.F., Attisano, L., Wrana, J.L.,
1998. SARA, a FYVE domain protein that recruits Smad2 to the
TGFbeta receptor. Cell 95, 779–791.
Turing, A.M., 1952. The chemical basis of morphogenesis. Philos. Trans.
R. Soc. (London) 237, 37–72.
Uemura, T., Shepherd, S., Ackerman, L., Jan, L.Y., Jan, Y.N., 1989. Numb,
a gene required in determination of cell fate during sensory organ
formation in Drosophila embryos. Cell 58, 349–360.
Wiellette, E.L., McGinnis, W., 1999. Hox genes differentially regulate
Serrate to generate segment-specific structures. Development 126,
1985–1995.
M. Gonzalez-Gaitan / Mechanisms of Development 120 (2003) 1265–1282 1281
Willert, K., Brown, J.D., Danenberg, E., Duncan, A.W., Weissman, I.L.,
Reya, T., et al., 2003. Wnt proteins are lipid-modified and can act as
stem cell growth factors. Nature 423, 448–452.
Wolpert, L., 1969. Positional information and the spatial pattern of cellular
differentiation. J. Theor. Biol. 25, 1–47.
Wrana, J.L., Attisano, L., Wieser, R., Ventura, F., Massague, J., 1994.
Mechanism of activation of the TGF-beta receptor. Nature 370, 341–347.
Wurmser, A.E., Gary, J.D., Emr, S.D., 1999. Phosphoinositide 3-kinases
and their FYVE domain-containing effectors as regulators of vacuolar/
lysosomal membrane trafficking pathways. J. Biol. Chem. 274,
9129–9132.
Zeng, C., Younger-Shepherd, S., Jan, L.Y., Jan, Y.N., 1998. Delta and
Serrate are redundant Notch ligands required for asymmetric cell
divisions within the Drosophila sensory organ lineage. Genes Dev. 12,
1086–1091.
Zhu, H., Kavsak, P., Abdollah, S., Wrana, J.L., Thomsen, G.H., 1999. A
SMAD ubiquitin ligase targets the BMP pathway and affects embryonic
pattern formation. Nature 400, 687–693.
M. Gonzalez-Gaitan / Mechanisms of Development 120 (2003) 1265–12821282