Morphogen gradients provide positional cues for cell fate specification and tissue patterning during embryonic development. One important aspect of morphogen function, the mechanism by which long-range signalling occurs, is still poorly understood. In Xenopus, members of the TGF-β family such as the nodal-related proteins and activin act as morphogens to induce mesoderm and endoderm. In an effort to understand the mechanisms and dynamics of morphogen gradient formation, we have used fluorescently labelled activin to study ligand distribution and Smad2/Smad4 bimolecular fluorescence complementation (BiFC) to analyse, in a quantitative manner, the cellular response to induction. Our results indicate that labelled activin travels exclusively through the extracellular space and that its range is influenced by numbers of type II activin receptors on responding cells. Inhibition of endocytosis, by means of a dominant-negative form of Rab5, blocks internalisation of labelled activin, but does not affect the ability of cells to respond to activin and does not significantly influence signalling range. Together, our data indicate that long-range signalling in the early Xenopus embryo, in contrast to some other developmental systems, occurs through extracellular movement of ligand. Signalling range is not regulated by endocytosis, but is influenced by numbers of cognate receptors on the surfaces of responding cells.
- Nodal-related proteins
- Bimolecular fluorescence complementation (BiFC)
The mesoderm of the amphibian embryo forms from the equatorial region of the late blastula in response to signals derived from the vegetal hemisphere of the embryo (Heasman, 2006). These signals include members of the transforming growth factor type β (TGF-β) family such as Vg1, activin, the nodal-related proteins Xnr1, 2, 4, 5 and 6, and derrière (Birsoy et al., 2006; Jones et al., 1995; Joseph and Melton, 1997; Piepenburg et al., 2004; Smith, 1995; Sun et al., 1999; Takahashi et al., 2000; White et al., 2002). Two significant characteristics of these signals are that they can act at long range and that they behave as morphogens, eliciting different responses at different concentrations. These properties raise the question of how such molecules exert their long-range effects: what route do they take to traverse a field of responding cells?
This question has been addressed for TGF-β family members in several developing systems, and particularly in the Drosophila imaginal disc, where one proposal is that long-range signalling by Decapentaplegic (Dpp) occurs in this epithelial tissue by transcytosis (Entchev et al., 2000; Gonzalez-Gaitan and Jackle, 1999). According to this model, Dpp released by signalling cells would be taken up by adjacent cells by endocytosis, and after traversing these cells it would be released by exocytosis further away from the source, for the process then to be repeated. Although the data supporting transcytosis in Drosophila has been reinterpreted to suggest that Dpp exerts its long-range effects by diffusion (Belenkaya et al., 2004; Lander, 2007), endocytosis has been shown to play a role in regulating the range of Fgf8 signalling in the zebrafish neurectoderm (Scholpp and Brand, 2004). Another model involving endocytosis has been proposed for the transfer of Wingless (Wg), Hedgehog (Hh) and Dpp in the epithelium of the Drosophila imaginal wing disc, where morphogens have been suggested to exert long-range effects by means of cellular extensions (Hsiung et al., 2005; Incardona et al., 2000).
In this paper we investigate the dynamics of morphogen gradient formation in the Xenopus embryo and the role of endocytosis in regulating signalling range and in the cellular response to induction. We conclude that activin exerts its long-range effects through an extracellular route, that signalling range is influenced by the density of cognate receptors expressed on the surface of responding cells, and that Rab5-mediated endocytosis plays no significant role in morphogenetic signalling, neither with respect to transmission of the signal across a field of responding tissue and nor with respect to the cellular response to induction.
MATERIALS AND METHODS
Xenopus embryos and manipulation
Xenopus embryos were obtained, injected, dissected and staged as described (Nieuwkoop and Faber, 1975; Tada et al., 1997). For animal cap assays, animal pole regions were transferred to agarose-coated dishes and cultured in 0.75× normal amphibian medium (NAM) (Slack, 1984) containing 0.2% bovine serum albumin (BSA). To investigate long-range signalling, animal pole regions were transferred to fibronectin-coated (10× dilution of 0.1% fibronectin from bovine plasma, Sigma) glass-bottomed dishes (MatTek) in 0.75× NAM, essentially as described (Williams et al., 2004). For `bead' experiments, Affi-Gel beads (Affi-Gel Blue Gel, Bio-Rad, 100-200 mesh) were incubated overnight with 1 mM Alexa488-activin protein at 4°C. For dissociated cell experiments, animal caps were dissociated in Ca2+- and Mg2+-free medium (75 mM Tris pH 7.5, 880 mM NaCl, 10 mM KCl, 24 mM NaHCO3) for 30-45 minutes at room temperature and were then transferred to 0.75× NAM containing 0.2% BSA before being treated with activin. Dissociated cells were seeded onto a fibronectin-coated or 0.75μ g/ml E-cadherin-coated (recombinant human E-cadherin, R&D Systems) (Ogata et al., 2007) glass bottom dish (MatTek) in 0.75× NAM containing 0.2% BSA in the presence or absence of 1 μg/ml Alexa488-activin or 5 μg/ml transferrin. For colocalisation assays, dissociated cells were derived from animal pole regions of uninjected embryos or embryos previously injected at the 1-cell stage with RNA encoding Rab4-, Rab5-, Rab7-, Rab11- or Hrs-Cherry. In some cases cells derived from uninjected embryos were treated with LysoTracker Red (Molecular Probes) for 1 hour before washing and imaging.
Real-time RT-PCR using primers specific for Xbra, goosecoid, chordin, Fgf8 and ornithine decarboxylase (Odc) was carried out as described (Piepenburg et al., 2004). Primers for histone H4 were as described (Niehrs et al., 1994). All values were normalised to the level of Odc or histone H4 in each sample.
cDNAs encoding activin βB, Xnr1, Xnr2, Xnr4, Smad2-VC155, Smad4-VN154-m9, histoneH2B-CFP, GFP-Gap43, Rab5S43N (kind gift from M. Gonzalez-Gaitan, University of Geneva, Geneva, Switzerland), mCherry-xlRab4, mCherry-dmRab5, mCherry-dmRab7, mCherry-xlRab11 and mCherry-xlHrs were all cloned in the expression vector pCS2+. Xenopus laevis Rab4, Rab11 and Hrs cDNAs were obtained as IMAGE clones; mCherry cDNA was the kind gift from Roger Tsien (Howard Hughes Medical Institute and University of California, San Diego, La Jolla, CA, USA). All such constructs were linearised with NotI and transcribed in vitro using SP6 RNA polymerase and the mMESSAGE mMACHINE kit (Ambion). GPI-CFP, mouse ActRIIB and Xenopus laevis DNActRIIB were cloned in the vector pSP64T BX, linearised with EcoRI and transcribed with SP6 RNA polymerase. Human dynaminK44E (kind gift from John Gurdon, Wellcome Trust/Cancer Research UK Gurdon Institute and Department of Zoology, University of Cambridge, Cambridge, UK) in pGEMHE was linearised with NheI and transcribed with T7 RNA polymerase. Smad2-VC155, Smad4-VN154-m9, histoneH2B-CFP, GPI-CFP and GFP-Gap43 were as described (Saka et al., 2008; Saka and Smith, 2007; Williams et al., 2004).
Labelled activin A preparation
Recombinant purified human activin A was labelled with Alexa Fluor 488 as follows: 2 mg of lyophilised activin A (154 nmol of protomers) was dissolved in 500 μl of 100 mM sodium phosphate buffer at pH 7.4 with 20% acetonitrile. Neutral pH was chosen to promote preferential labelling at the N-terminus of the protein. Then 0.2 mg (311 nmol) of acetonitrile-solubilised Alexa Fluor 488 carboxylic acid succinimidyl ester (Invitrogen) was added to the protein and the reaction allowed to proceed for 1 hour in the dark. The sample was acidified with trifluoroacetic acid (TFA) and loaded onto a Vydac 214TP510 C4 reversed-phase column and eluted with a gradient of acetonitrile in 0.1% TFA. Peak fractions corresponding to labelled activin dimer were lyophilised under vacuum, solubilised in water, divided into four pools based on the level of labelling and stored at -20°C. Protein concentration was determined by quantitative amino acid analysis and the level of fluorophore incorporation was measured spectrophotometrically using a molar absorption coefficient for Alexa Fluor 488 of 71,000 at 500 nm. On average each activin dimer contained 0.7-1.4 fluorophores and mass-spectrometric analysis of the labelled samples showed at most three labels per dimer (data not shown).
Images in Figs 1, 5, 7, and supplementary material Figs S2A-E and S3 were taken using a Perkin Elmer Spinning Disc confocal microscope with a Zeiss Axiovert 200M inverted microscope and a Hamamatsu ORCA ER camera. CFP protein was excited at 440 nm, VENUS BiFC at 514 nm, Alexa488 at 488 nm and Alexa594 at 568 nm. Pictures were acquired using UltraVIEW ERS software. Images in Figs 2, 3, 4, 6, 8 and supplementary material Fig. S2F-H were taken using an Olympus inverted FV1000 confocal microscope. CFP protein was excited at 458 nm, VENUS BiFC at 515 nm, mCherry at 564 nm and Alexa488 at 488 nm. Pictures were acquired using FluoView software. All confocal pictures were taken with a 40× oil objective and supplementary material Figs S2A-E and S3 represent a merged z-stack consisting of 15 slices, each 1 μm thick.
Fluorescence was quantified using Volocity software and is presented as the mean values of manually drawn regions of interest (ROIs) identified by referring to the coexpressed membrane marker CFP-GPI (Fig. 2) or by automatic selection of all CFP-histoneH2B-positive nuclei and normalised to CFP-histone marker (Fig. 3).
Rapid extracellular spreading of Alexa488-activin is followed by slower internalisation
The most direct approach to investigate the role of endocytosis in morphogenetic signalling is to use fluorescently labelled proteins and live cell imaging. In past work we have made use of an EGFP-Xnr2 fusion protein to follow the passage of a TGF-β family member through Xenopus animal pole explants (Williams et al., 2004), and found no evidence for ligand internalisation. However, it is possible that this approach is not sufficiently sensitive, and in addition, without accurate knowledge of ligand concentrations, it is difficult to obtain quantitative results. In an effort to address these concerns, we have instead labelled activin protein with Alexa Fluor 488. Activin can act as a potent long-range morphogen (Jones et al., 1996) and our experiments show that this labelled activin retains ∼50% of its biological activity (Fig. 1A) and that it is internalised by isolated Xenopus animal pole blastomeres in a specific manner (Fig. 1B-F). Under our experimental conditions we can readily visualise an extracellular concentration of Alexa488-activin of 250 ng/ml and lower concentrations might also be detectable (see Fig. S1A-E in the supplementary material).
To investigate the ability of this labelled activin to traverse a field of responding cells, we soaked Affi-Gel (Bio-Rad) beads in Alexa488-activin and introduced them into animal pole regions that had been allowed to adhere to a fibronectin-coated substrate (Williams et al., 2004). To expand the space available for ligand movement, the animal pole regions were juxtaposed with two additional animal caps (Fig. 2A). Alexa488-activin was distributed in a diffuse manner in the extracellular space 1 hour after introducing the bead, with little fluorescence visible within cells (Fig. 2B,E,H). Fluorescent activin was also located in discrete aggregates within cells 1 hour later, although extracellular levels were still higher than intracellular levels (Fig. 2C,F,I). The number of internalised Alexa488-activin aggregates increased further over the next hour, although the amount of extracellular activin, derived from the implanted bead, decreased (Fig. 2D,G,J).
This temporal analysis of activin distribution, in which the appearance of extracellular ligand precedes that of internalised material, is consistent with the idea that activin can spread from its source via an extracellular route.
Smad2/4 bimolecular fluorescence complementation provides a direct read-out of long-range signalling by TGF-β family members
In an effort to visualise a direct response to long-range TGF-β signalling, we have turned to Smad2-Smad4 bimolecular fluorescence complementation (Smad2/4-BiFC). This approach has already been used to visualise Smad signalling in cells of the Xenopus embryo (Saka et al., 2007), and it provides a direct, quantitative and rapid read-out of activin-like signalling, with a better signal-to-noise ratio than obtained by monitoring the nuclear translocation of GFP-Smad2 (Bourillot et al., 2002; Grimm and Gurdon, 2002; Kinoshita et al., 2006). Animal pole explants were therefore derived from embryos co-injected with mRNAs encoding (1) Smad2/4-BiFC constructs (Saka et al., 2007); (2) activin or Xnr1; and (3) fluorescent markers for membrane and for chromatin (CFP-GPI and CFP-histoneH2B, respectively). These pieces of tissue were juxtaposed with animal pole tissue derived from embryos co-injected with RNAs encoding the Smad2/4-BiFC constructs and CFP-histoneH2B (Fig. 3A) and the conjugates were cultured on a fibronectin-coated surface for 4 hours before being viewed live under the confocal microscope. The ability of activin and Xnr1 to activate gene expression at long range was confirmed by RT-PCR analysis of animal pole regions that were separated after 4 hours of culture (Fig. 3B).
In the absence of TGF-β ligands, Smad BiFC activation was not detectable in signalling or responding cells (Fig. 3C,D), but in the presence of activin or Xnr1, nuclear BiFC fluorescence was observed in both tissues (Fig. 3E-H). In the responding tissue, levels of nuclear Smad2/4-BiFC fluorescence decreased with increasing distance from the signalling cells, and higher concentrations of injected activin RNA increased the range of BiFC activation (Fig. 3I). Quantitation of experiments such as these is complicated by the fact that there is significant `noise' in the system; Smad2/4-BiFC levels in adjacent cells can differ significantly. Nevertheless, timecourse experiments suggest that the range of activin signalling does not expand significantly between 1.5 and 3 hours after animal cap juxtaposition, but that the intensity of Smad BiFC does increase (Fig. 3J and see Fig. S2F-H in the supplementary material). These observations indicate that the establishment of a stable activin gradient occurs within 90 minutes. They also suggest that cells can increase their level of response over a longer period than this, although this observation may derive in part from the stability of Smad2/4-BiFC complexes (Saka et al., 2007).
Together, our results indicate that Smad2/4-BiFC provides a fast and direct means for detecting long-range signalling by members of the TGF-β family. Additional experiments revealed that other nodal-related proteins such as Xnr2 and Xnr4 also induce nuclear Smad BiFC activation, albeit less efficiently than activin and Xnr1 (see Fig. S2 in the supplementary material).
Increasing numbers of cell surface receptors cause signalling range to decrease
In an effort to ask to what extent receptor-mediated endocytosis influences activin signalling range, we overexpressed wild-type or truncated forms of the type IIB activin receptor (ActRIIB) in tissue that is positioned between a source of activin and a population of responding cells. Activin, like other TGF-β family members, signals by interacting first with a type II receptor, which then associates with and phosphorylates a type I receptor serine/threonine kinase. This activated type I receptor goes on to phosphorylate the receptor-regulated Smads 2 or 3, which associate with Smad4 and enter the nucleus to regulate transcription (Armes and Smith, 1997; Wu and Hill, 2009).
Overexpression of both the wild-type activin receptor ActRIIB and a truncated form lacking only the intracellular domain (DNActRIIB) caused Alexa488-activin to accumulate around and within cells close to the source of the signal (Fig. 4) and long-range signalling, monitored by Smad2/4-BiFC, was not observed (DNActRIIB) or was significantly reduced (ActRIIB; see Fig. S3 in the supplementary material). The increased internalisation of Alexa488-activin caused by expression of the activin receptors suggests that this internalisation is a specific process rather than non-specific phagocytosis of extracellular material.
Overexpression of the wild-type activin type II receptor does not lead to increased signalling activity in responding cells, as judged by the intensity of Smad2/4-BiFC (see Fig. S3 in the supplementary material and data not shown). It is possible that levels of type I, rather than type II, receptor are limiting in these cells, because overexpression of the type I receptor Thickveins in Drosophila does sensitise cells to levels of Dpp (Lecuit and Cohen, 1998). Future experiments will ask how the downregulation of activin receptors influences activin signalling range.
The failure of increased receptor density to extend signalling range suggests that activin does not exert its long-range effects by transcytosis. Indeed, the dramatic reduction in signalling range suggests that receptor-mediated endocytosis in Xenopus restricts the passage of activin, as is also observed for Fgf8 in the developing zebrafish neurectoderm (Scholpp and Brand, 2004).
Activin does not spread via transcytosis in Xenopus blastula cells
To investigate in more detail whether internalised activin can transfer from one cell to another, we designed a cell mixing assay in which cells that had previously been treated with activin were mixed with untreated cells. In the course of these experiments, animal pole blastomeres derived from embryos at the late blastula stage were dissociated and incubated in Alexa488-activin before being acid-washed to remove any adherent ligand. These cells were mixed with dissociated cells that had not been incubated with activin and they were allowed to aggregate for at least 3 hours before imaging (Fig. 5A). The two populations could be distinguished by the expression of different fluorescent cell markers, and both were expressing our Smad2/4-BiFC constructs (Fig. 5A).
Under these conditions, we were unable to observe the transfer of labelled activin from treated to untreated cells and nor could we observe nuclear Smad2/4-BiFC in untreated cells (Fig. 5B-H). As a control, to ensure that cells remained healthy and susceptible to newly exocytosed activin throughout the procedure, two untreated populations of cells were mixed and treated with Alexa488-activin during aggregation (Fig. 5A). These cells internalised fluorescent activin and showed nuclear accumulation of Smad2/4-BiFC (Fig. 5I-L). These experiments suggest that passage of activin via transcytosis does not occur in Xenopus blastomeres.
Internalised Alexa488-activin associates with Rab5-containing endosomes and then with lysosomes
In an effort to investigate the fate of internalised Alexa488-activin, we next studied its intracellular localisation in Xenopus animal pole blastomeres. Ligand-receptor complexes of TGF-β family members have been suggested to associate with clathrin-coated endosomes that fuse with Rab5-positive early endosomes shortly after budding from the cytoplasmic membrane (Zerial and McBride, 2001). We investigated this process in the early Xenopus embryo by isolating animal pole blastomeres from embryos expressing tagged endocytosis markers. Such blastomeres were incubated in Alexa488-activin for 20 minutes and examined at intervals thereafter. After 10 minutes, 50% of intracellular Alexa488-activin aggregates were associated with Rab5, a marker of early endosomes (Fig. 6A-C,P), or Rab7, a marker of late endosomes or multi-vesicular bodies (MVBs). Over 60% of aggregates colocalised with Rab4, which is expressed in early endosomes and is involved in degradation and in the fast recycling pathway (Sonnichsen et al., 2000), or Hrs, which marks the degradation pathway from early endosomes onwards (McCaffrey et al., 2001; Saksena et al., 2007; Williams and Urbe, 2007). These figures decreased to ∼20% for Rab5 and less than 40% for Rab4 and Rab7 over the next 30 minutes, whereas colocalisation with Hrs increased to over 80% (Fig. 6D-F,P). By 3.5 hours, 93% of Alexa488-activin particles were associated with lysosomes, as revealed by the colocalisation of activin-Alexa488 with LysoTracker Red (Fig. 6G-O).
Although Rab11 can be detected with Rab7 on MVBs (Bottger et al., 1996), this is predominantly a marker of recycling vesicles (Sonnichsen et al., 2000). At all times tested, only ∼10% of Alexa488-activin particles associated with Rab11 (Fig. 6P). Together, these observations suggest that the great majority of intracellular activin is targeted for degradation rather than for transcytosis.
Ligand internalisation is not required for gene induction or for long-range signalling
In a final effort to investigate the role of endocytosis in long-range signalling in the Xenopus embryo, we turned to inhibitors of endocytosis. The results described above indicate that internalised activin associates with Rab5, so we have made use of Rab5S43N, a dominant-negative form of Rab5. Animal pole blastomeres derived from embryos injected with RNA encoding Rab5S43N failed to internalise Alexa488-activin (Fig. 7A-C) and, in an additional assay, the internalisation of transferrin into animal pole blastomeres expressing the transferrin receptor was also attenuated (Fig. 7D,E). Inhibition of activin uptake was more effective than that of transferrin (Fig. 7F), perhaps because the transferrin receptor was overexpressed to high levels. Other inhibitors of endocytosis, including dynaminK44E and dynaminK535A (dominant-negative versions of dynamin), phenylarsine oxide and monodansyl cadaverine, were less effective than Rab5S43N or were too toxic (see Fig. S4 in the supplementary material and data not shown).
Our first series of experiments asked whether endocytosis is required for the induction of gene expression by activin. This is a significant issue because there is no consensus concerning the necessity for endocytosis for TGF-β signalling; some investigations have suggested that endocytosis is essential (Hu et al., 2008; Jullien and Gurdon, 2005; Kinoshita et al., 2006; Penheiter et al., 2002; Runyan et al., 2005), whereas others indicate that TGF-β or activin signalling can occur from the cytoplasmic membrane (Chen et al., 2009; Lu et al., 2002; Panopoulou et al., 2002; Zhou et al., 2004; Zwaagstra et al., 2001). In our experiments, we treated animal pole regions derived from embryos expressing Rab5S43N with activin and went on to measure the activation of target genes, including Gsc, Xbra and chordin, at different developmental stages. The ability of the dominant-negative form of Rab5 to inhibit the internalisation of activin was confirmed in parallel experiments (Fig. 7A-F and data not shown). In no case was target gene expression inhibited by Rab5S43N. Indeed, expression of Xbra was slightly elevated after stage 10.5 in blastomeres in which Rab5 function was inhibited, perhaps as an indirect effect of endocytosis-dependent signalling events. Interestingly, a similar enhancement of TGF-β signalling has been observed in Mv1Lu cells treated with inhibitors of clathrin-dependent endocytosis (Chen et al., 2009). Together, these results suggest that in Xenopus animal pole region endocytosis is not required for the activation of gene expression by activin (Fig. 7G and see Fig. S4 in the supplementary material).
At first sight our results using Rab5S43N are at odds with reports that dynaminK44E can inhibit activin signalling in Xenopus embryonic tissue (Jullien and Gurdon, 2005; Kinoshita et al., 2006). In searching for an explanation, we first note that the two inhibitory constructs target different components of the endocytic pathway. In addition, whereas previous work tested the efficacy of dynaminK44E by monitoring the internalisation of exogenously expressed activin receptors, or of labelled transferrin via an exogenously expressed transferrin receptor (Jullien and Gurdon, 2005; Kinoshita et al., 2006), our work demonstrates that dynaminK44E (in contrast to Rab5S43N) has little effect on the uptake of Alexa488-activin via endogenous receptors (data not shown). Finally, our quantitative RT-PCR experiments revealed that dynaminK44E causes only a slight decrease in the expression of Xbra in response to activin, with no effect on the expression of goosecoid (see Fig. S4C in the supplementary material and data not shown). Similar results were obtained using Smad2/4-BiFC, which provides single-cell resolution of the response to activin with a higher signal-to-noise ratio than is obtained with Smad2-GFP imaging. Together, these data are consistent with our conclusion that endocytosis is not required for the cellular response to activin.
We next asked whether endocytosis is required for long-range signalling. In the first experiment, animal pole tissue expressing Rab5S43N was positioned between an animal pole region containing a bead soaked in Alexa488-activin and an untreated animal pole region. Conjugates were cultured for 4 hours before the distribution of fluorescent activin was analysed. In control experiments, and as previously described, Alexa488-activin was detectable many cell diameters from the activin source, with ligand present both in the extracellular space and within cells (Fig. 2C,D and Fig. 8B). Fluorescent activin was also able to traverse cells expressing Rab5S43N, but in such cases Alexa488-activin was exclusively extracellular (Fig. 8A).
In another set of experiments we examined the influence of endocytosis on activin signalling range by juxtaposing animal pole regions derived from embryos expressing activin mRNA with responding tissue expressing Rab5S43N. Both groups of cells also expressed Smad2/4-BiFC constructs, which confirmed that activin can signal in cells in which endocytosis is inhibited and again revealed that activin can exert its effects at long range even in the absence of endocytosis (Fig. 8B-G).
Mesoderm formation in the early embryo of Xenopus laevis requires the activities of at least eight distinct members of the TGF-β family, all of which are thought to act in a concentration-dependent manner, and many of which can act at long range (Agius et al., 2000; Green, 2002; Sun et al., 1999; Takahashi et al., 2000). Proper mesoderm formation requires that the actions of these morphogens are coordinated such that concentration gradients are generated in a reliable and reproducible manner. In this paper we study the way in which these gradients are established.
Activin travels through an extracellular route
Our results suggest that activin travels through an extracellular route that does not involve transcytosis. Thus, Alexa488-activin can be detected extracellularly remote from its source within 1 hour, well before it can be visualised intracellularly, at about 2 hours (Fig. 2). In addition, animal pole blastomeres that had been preloaded with Alexa488-activin could not pass ligand to adjacent unloaded cells, nor could they induce Smad2/4-BiFC in such cells (Fig. 5). And finally, although inhibition of Rab5-mediated endocytosis does prevent internalisation of Alexa488-activin (Fig. 7A-C,F and Fig. 8A), it does not prevent its passage through responding tissue (Fig. 8A) and nor does it significantly affect its signalling range (Fig. 8C-H) or the cellular response to induction (Fig. 7G, see Fig. S4A,B in the supplementary material and below). Indeed, our results suggest that internalised activin is destined for lysosomes rather than for re-secretion and long-range signalling (Fig. 6). These results are consistent with some aspects of previous work (Kinoshita et al., 2006), but extend it by visualising activin ligand directly.
Our efforts to fit the extracellular distribution of Alexa488-activin to an exponential or power trend line have failed, perhaps because the bead used to supply the activin does not represent a continuous source (see Fig. S1 in the supplementary material and data not shown). We do observe, however, that the distribution of internalised activin fits a power trend line to a good approximation from 2 hours onwards. The elevated decay of activin close to the source of the ligand suggests that the rate of intracellular degradation exceeds the rate of uptake, because we show that significant amounts of activin do not leave the cell after endocytosis (Figs 5 and 6).
Our conclusion that long-range signalling in Xenopus occurs through an extracellular route differs from the suggestion made for the Drosophila imaginal wing disc that Dpp might traverse cells by transcytosis (Entchev et al., 2000; Gonzalez-Gaitan and Jackle, 1999). We note, however, that the Drosophila imaginal disc consists of a closely packed polarised epithelium, whereas cells in the Xenopus blastula are arranged as a looser mesenchyme. Contacts in the Xenopus tissue are likely to be less stable and fewer in number than in the imaginal disc, so that long-range signalling by transcytosis is likely to be much less efficient in this tissue.
Receptor density but not Rab5-mediated endocytosis influences signalling range
In some respects our results are consistent with those of Scholpp and Brand (Scholpp and Brand, 2004), who find that inhibiting internalisation of Fgf8 in the neurectoderm of the zebrafish extends its signalling range, while elevating internalisation reduces it. Consistent with these results, our data show that an increase of the ligand-receptor interaction surface due to overexpression of an activin receptor causes the accumulation of ligand inside and at the surface of responding cells, and this prevents its movement further into responding tissue (Fig. 4). Similarly, in Drosophila, levels of a type I receptor limits the range of Dpp signalling (Lecuit and Cohen, 1998). Together, our data remain consistent with a model in which long-range signalling by morphogens occurs by simple extracellular diffusion (Belenkaya et al., 2004; Lander et al., 2002).
However, in contrast to Scholpp and Brand (Scholpp and Brand, 2004), we find that inhibition of activin internalisation does not significantly extend its signalling range (Fig. 8G,H). One explanation might be that the two systems, zebrafish neurectoderm and Xenopus animal pole tissue, differ with respect to the space available for ligand distribution. In particular, our system provides a space that is effectively infinite, because the morphogen can eventually diffuse beyond the edges of the explant. The significance of this extended space is under investigation, and we also note that the signalling ranges of different ligands (Fgf8 and activin) in different tissues (neurectoderm and animal pole tissue) may well be subject to different types of regulation.
Receptor-mediated endocytosis is not required for gene activation
Our experiments also reveal that Rab5-mediated endocytosis is not required for the activation of the activin signal transduction pathway, as revealed both by Smad2/4-BiFC (Fig. 8C-H) and by the induction of gene expression (Fig. 7G and see Fig. S4A,B in the supplementary material). The elevation of Xbra expression associated with the inhibition of Rab5 activity (see Fig. S4B in the supplementary material) is likely to be due to an indirect effect.
There is no consensus in the literature about the requirement for endocytosis in growth factor function. There are likely to be differences between different ligands and different cell types, and the point at which the pathway is inhibited might also be significant. Consistent with our results, which show that Rab5S43N does not inhibit gene induction by activin in Xenopus animal pole regions (Fig. 7G), the inhibition of endocytosis by RN-tre, dynaminK44A (a dominant-negative form of dynamin) and an antisense morpholino oligonucleotide directed against Rab5 does not prevent gene activation in response to Fgf8 (Scholpp and Brand, 2004). Our results differ, however, from those of Jullien and Gurdon, who report that dynaminK44E inhibits activin-induced induction of Xbra and eomesodermin in Xenopus blastomeres (Jullien and Gurdon, 2005). As discussed above, we do not yet understand the reason for this apparent discrepancy, which is under investigation.
Finally, we noted in the course of our experiments that Alexa488-activin occasionally accumulated at the site of membrane scission following cytokinesis (20-30% of cells; Fig. 1B; see Movie 1 in the supplementary material). A similar accumulation of transferrin has been suggested to occur as a result of the directed transport of recycling vesicles carrying receptor-bound ligand to the midbody region (Schweitzer et al., 2005). This may ensure the equal distribution of signalling complexes between daughter cells (Bokel et al., 2006). Cells lacking functional Rab11, a marker of recycling vesicles, fail to complete cytokinesis (Yu et al., 2007); a similar effect is observed following overexpression of Cherry-Rab11 (see Movie 1, left cell in the supplementary material).
Supplementary material for this article is available at http://dev.biologists.org/cgi/content/full/136/16/2803/DC1
We thank all present and former members of our laboratory, especially Elizabeth Callery and Kevin Dingwell, for their helpful comments. We are also grateful to Mike Gilchrist (Gurdon Institute) for discussion and to Marcos Gonzalez-Gaitan and Roger Tsien for cDNA constructs. This work is supported by the EU sixth framework project `EndoTrack' (FP6 Grant LSHG-CT-2006-019050), by a Wellcome Trust Programme Grant awarded to J.C.S., and by the Foundation for Science and Technology (FCT), Portugal. A.I.H. is a student of the Gulbenkian PhD Program in Biomedicine, Portugal. Deposited in PMC for release after 6 months.
- Accepted June 12, 2009.
- © 2009.