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Experimental Cell Research 281, 101–106 (2002) doi:10.1006/excr.2002.5650 Thrombin Activation of S-Phase Reentry by C ultured Pigmented E pithelial C ells of Adult N ewt Iris András Simon 1,2 and Jeremy P. Brockes Department of Biochemistry and Molecular Biology, University College London, London, WC1E 6BT United Kingdom; and Medical Nobel Institute, Department of Cell and Molecular Biology, Karolinska Institute, Stockholm, Sweden Following local injury or tissue removal, regeneration in urodele amphibians appears to be dependent on cell cycle reentry and dedifferentiation of postmitotic, terminally differentiated cells in the remaining tissues. Regeneration of the lens of the eye occurs by the dedifferentiation of pigmented epithelial cells (PEC) of the iris and their subsequent transdifferentiation into lens cells. A key question is how cell cycle reentry is regulated. Here we demonstrate that thrombin activates S-phase reentry of newt PEC in vitro. Based on these findings, and on previous experiments showing that newt skeletal myotubes reenter the cell cycle following thrombin stimulation, we suggest that thrombin is a critical signal for initiation of vertebrate regeneration. © 2002 Elsevier Science (USA) INTRODUCTION Urodele amphibians, such as newts and axolotls, have a unique capacity among vertebrates to regenerate their body parts as adults. While loss or degeneration of the neuroretina and other ocular structures leads to visual handicap and eventually blindness in most vertebrates, a newt can regenerate its lens and neuroretina. Other newt structures which can be replaced after injury include the upper and lower jaws, spinal cord, parts of the central nervous system, the cardiac musculature, and the intestine [1, 2]. Several studies emphasize the role of the plasticity of the differentiated state during amphibian regeneration and show that the progenitor cells of the regenerate are derived from postmitotic, differentiated cell types (for a review see [3]). Multinucleated skeletal muscle cells reenter the cell cycle and undergo fragmentation into proliferating, cycling progeny cells during limb and tail regeneration in urodeles. These prog1 Present address: Medical Nobel Institute, Department of Cell and Molecular Biology, Karolinska Institute, Stockholm, Sweden. 2 To whom correspondence and reprint requests should be addressed. Fax: 46(0)8308374. E-mail: [email protected]. eny cells contribute to the growth zone or blastema, from which the cells of the regenerate originate [4 – 8]. Similarly, regeneration of the heart depends on cell cycle reentry and proliferation of cardiomyocytes in the vicinity of the injury [9]. Regeneration of ocular structures such as the lens and neuroretina depends on transdifferentiation. Upon removal of the lens, pigmented epithelial cells (PEC) in the dorsal margin of the iris enter S phase, lose their pigmentation, and give rise to a new lens. Transdifferentiation to lens is confined normally to PEC of the pupillary margin of the dorsal iris and the new lens does not arise from the ventral iris [10]. The molecular mechanisms that induce cells to leave the postmitotic arrest have long remained enigmatic. Recently it was shown that the postmitotic arrest of newt skeletal myotubes in culture can be undermined by stimulating them with serum [11]. The active component in serum is not a known protein growth factor but an as yet unidentified molecule, which is activated by thrombin but which is distinct from the protease [12]. Thus, a subthreshold concentration of serum can be activated by digestion with thrombin, followed by inhibition of residual protease activity. The thrombin-derived activity, which leads to cell cycle reentry of the newt myotubes, is inactive on mouse myotubes, although it is present in sera from various mammalian sources [12, 13]. It is appealing to speculate that following injury, the activation of thrombin generates a signal, which newt cells can transduce and which evokes a key cellular response in regeneration. Here we have addressed the question of whether the thrombin-derived activity may represent a common signal for cells involved in a different context of regeneration. Since cell cycle reentry of PEC is the first step in lens regeneration, we established a culture model in which the PEC are quiescent but respond to appropriate molecules that can induce cell cycle reentry. We found that the thrombin-derived activity is able to induce S-phase reentry of PEC in vitro. 101 0014-4827/02 $35.00 © 2002 Elsevier Science (USA) All rights reserved. 102 SIMON AND BROCKES FIG. 1. Morphology of PEC in culture. (A and D) Phase-contrast image of PEC at 20- and 40-fold magnifications, respectively. (B and E) DAPI (blue) staining of the nuclei at 20- and 40-fold magnifications, respectively. (C and F) BrdU staining of nuclei in S-phase (red) at 20and 40-fold magnifications, respectively. Scale bar, 50 !m THROMBIN AND S-PHASE REENTRY 103 FIG. 2. S-phase reentry of PEC induced by increasing concentration of FCS. Bars represent the averages of three independent wells in a representative experiment. Dots indicate the results in the individual wells. MATERIAL AND METHODS Animals. Red spotted newts, Notophthalmus viridescens, were purchased from Charles Sullivan Co. (TN). Animals were kept in tap water at 19°C and fed once a week. Preparation of PEC. Animals were anesthetized by immersion in 0.1% MS 222 (Sigma) dissolved in tap water. The eyeballs were removed and collected in a tissue culture dish containing PBS adjusted to amphibian osmolarity. The eyeballs were washed in 70% ethanol for 2 min and transferred to Leibowitz-15 (L-15) medium (Gibco), adjusted to amphibian osmolarity, and supplemented with 0.5% bovine serum albumin (BSA), penicillin/streptomycin, and Lglutamine. Corneal cells were removed and an anterior eye cup was created by cutting the eyeball along the iris. The lens was removed and the iris rings were placed in L-15 medium containing 0.5% BSA and 0.5% dispase grade II (La Roche). If dorsal and ventral cells were analyzed separately, the iris rings were cut into dorsal and ventral halves at this stage. The tissues were incubated at 25°C for 4 h and the sheet of PEC was separated from the underlying stromal cells. Dissociation of the PEC sheet was achieved by incubation with 0.25% trypsin–EDTA solution for 10 min at room temperature. Trypsin was diluted 1/20 in L-15 medium containing 0.5% BSA, and the cells were centrifuged at 100g for 5 min. Cells were resuspended in L-15 medium containing 0.5% BSA, and approximately 600 cells were plated onto collagen type IV- (Sigma) coated wells in 96-well plates. Thirty to fifty percent of the plated cells attached and spread. With this method over 99% of the cells were PEC. S-phase reentry assay. Seven days after plating, the cells were shifted to L-15 medium containing various concentrations of fetal calf serum (FCS; Gibco; Lot F40F8814) with or without thrombin or additional growth factors. After 3 days, bromodeoxyuridine (BrdU; La Roche) was added to a final concentration of 10 !M. After 18 –20 h the cells were fixed for 30 s in 2% paraformaldehyde and postfixed for 5 min in ice-cold methanol. To test the effect of growth factors, medium containing 0.25% FCS was supplemented with 40 ng/ml purified mouse EGF (Collaborative Research), human recombinant FGF-2 (Gibco; both factors are kind gifts from Professor Jonas Frisén), PDGF-C (a kind gift from Professor Ulf Eriksson), or all three growth factors simultaneously. The effect of thrombin was assayed in the presence of 0.25% FCS and 100 !g/ml crude preparation of bovine thrombin (Calbiochem). The effect of the thrombinderived activity was analyzed essentially as described in [12]. Briefly, medium containing 1% FCS was incubated with purified bovine thrombin (Enzyme Research Laboratories) for 24 h at 25°C. Thrombin was inactivated using a 50-fold molar excess of D-Phe-ProArg chloromethyl ketone (PPACK; Sigma). The activated medium containing 1% FCS was diluted to a final concentration of 0.25% FCS and added to cells. In control experiments PPACK and purified thrombin were added simultaneously in order to prevent activation. Thrombin activity was measured spectrophotometrically using Chromosyme TH (La Roche) as substrate according to the manufacturer’s recommendations. Thrombin activity was completely inhibited by PPACK. Immunocytochemistry and image analysis. BrdU staining was performed as described [11] and visualized using Alexa 546-conjugated anti-mouse IgG-specific secondary antibody (Molecular Probes). The nuclei were stained by DAPI. Cells were observed using a Nikon inverted microscope and pictures were captured by a color CCD camera. Data analysis. The data represent the average of results from three independent wells in a representative experiment. Between 90 and 300 cells were counted in each well. RESULTS AND DISCUSSION We first determined the conditions under which PEC are proliferating or quiescent. PEC were prepared and 104 SIMON AND BROCKES FIG. 3. Thrombin induces S-phase reentry of PEC. “Crude thr” indicates that medium containing 0.25% FCS was supplemented with a crude preparation of bovine thrombin as described under Material and Methods. “0.25% FCS non-act” indicates that medium containing 0.25% FCS was preincubated with both purified bovine thrombin and thrombin inhibitor for 24 h before addition to cells. “0.25% FCS act” indicates that medium containing 0.25% FCS was preincubated with purified thrombin for 24 h and thrombin activity was irreversibly inhibited before addition to cells. Bars represent the average of three independent wells in a representative experiment. Dots indicate the results in the individual wells. plated in serum-free medium. Figure 1 shows the morphology of the cells at two different magnifications. The cells are heavily pigmented, often display a hexagonal shape with clearly visible nuclei, and tend to attach to each other and to form islets (Figs. 1A, 1B, 1D, and 1E). In the presence of 10% FCS a substantial portion of PEC reenter S phase as assayed by BrdU incorporation (Figs. 1C and 1F). Most of the cells are quiescent in serum-free medium and as little as 1% FCS induced DNA replication in more than 20% of PEC (Fig. 2). The maximal level of S-phase reentry was observed in the presence of 10% FCS (Fig. 2). It should be noted that different sources of serum resulted in different levels of S-phase reentry (data not shown), although the overall pattern was the same as shown in Fig. 2. We therefore performed all experiments in the same batch of serum, as specified under Material and Methods. Next we asked whether thrombin could induce Sphase reentry as observed in the case of newt skeletal myotubes. We assayed the effect of a crude preparation of bovine thrombin in the presence of 0.25% FCS, since the background level at this serum concentration was relatively low. Crude thrombin resulted in a 6.5-fold increase in BrdU-positive cells compared to the control (Fig. 3). To test whether this effect of thrombin was direct or indirect, we activated FCS-containing medium with purified thrombin and inactivated the activity of the protease irreversibly by PPACK before addition to the cells [12]. As a control we used medium which was preincubated with thrombin in the presence of thrombin inhibitor. As shown in Fig. 3, thrombinactivated serum induced a 5.5-fold increase in the number of PEC that entered S-phase. The crude preparation of thrombin also induced S-phase reentry in serum-free medium, but to a lower extent compared to activation in the presence of serum (data not shown), suggesting that crude thrombin contains the thrombinderived activity identified by Tanaka et al. [12]. Lens regeneration in situ is dependent on the PEC of the dorsal margin of the iris, while ventral PEC do not participate in formation of the new lens [14]. To test whether this difference is correlated to thrombin responsiveness, we separated the iris into dorsal and ventral halves prior to the removal of PEC and seeded dorsal and ventral cells in separate wells. We did not find any difference between dorsal and ventral cells with respect to responsiveness to subthreshold concentration of serum, which was activated with pure throm- THROMBIN AND S-PHASE REENTRY 105 FIG. 4. Both dorsal and ventral PEC reenter S phase upon stimulation with thrombin-activated serum. Labels should be interpreted as in Fig. 3. Bars represent the average of three independent wells in a representative experiment. Dots indicate the results in the individual wells. FIG. 5. Growth factors induce S-phase reentry of PEC. “GF-MIX” indicates that all three growth factors were added to the medium. Bars represent the average of three independent wells in a representative experiment. Dots indicate the results in the individual wells. 106 SIMON AND BROCKES bin. Dorsal and ventral cells showed identical responses compared to control (Fig. 4). These results are in agreement with previous results by Eguchi et al. [15], which showed that both dorsal and ventral cells form lentoid bodies in vitro, despite the fact that only dorsal cells participate in lens regeneration in vivo. As serum also contains mitogenic growth factors, we wanted to see whether purified growth factors could induce S-phase reentry of PEC. We tested three different growth factors, EGF, PDGF-C, and FGF-2. All three induced cell cycle reentry to approximately the same level either alone (PDGF-C, 9.4-fold; FGF-2, 11fold; EGF, 10.7-fold), or in combination (10.5-fold), suggesting that PEC express receptors for these growth factors (Fig. 5). The phenomenon of Wolffian regeneration [16] is a demonstration of the reprogramming and transdifferentiation of a fully differentiated cell type, the PEC. Transdifferentiation begins with cell cycle reentry, and our results show that PEC respond to thrombin stimulation in culture in the same way as do skeletal myotubes. While the implications of this finding would still require extension from in vivo experiments, our results indicate that the thrombin-activated pathway may represent a common signal for postmitotic cells, which are reactivated during regeneration in newts. Various growth factors in addition to thrombin evoke DNA replication in PEC. This contrasts with the case of newt skeletal myotubes, which are refractory to growth factor stimulation [11, 12]. One simple interpretation of these data could be that PEC have receptors for these growth factors, whereas the myotubes have receptors for only the thrombin-activated factor. Nonetheless, these observations are in agreement with several previous studies which underline the role of mitogenic growth factors in proliferation and transdifferentiation of PEC to lens or lentoid bodies [17–19]. The culture system described here provides an opportunity for systematic analysis of the proliferative potential of PEC under different conditions. It may be useful in future experiments to investigate how cell cycle reentry and transdifferentiation are coupled to each other and how specific agents may influence their course. One important task for the future is also to determine whether thrombin is able to induce cells to complete the mitotic cycle. We are most grateful to Y. Imokawa for help with initial preparation of PEC and for helpful discussions. We thank K. Agata for advice on culture conditions, E. Tanaka for suggestions, S. Sandberg for comments on the manuscript, and J. Frisén and U. Eriksson for providing growth factors. The financial support from an MRC proReceived June 18, 2002 Revised version received August 15, 2002 Published online October 11, 2002 gram grant to J.P.B. and to A.S. from The Wenner–Gren Foundation, The Swedish Research Council, Carl Tryggers Stiftelse, Åke Wibergs Stiftelse, Magnus Bergvalls Stiftelse, and Stiftelsen Lars Hiertas Minne is greatly appreciated. REFERENCES 1. Stocum, D. L. (1995). “Wound Repair, Regeneration, and Artificial Tissues,” Landes, Austin, TX. 2. Wallace, H. (1981). “Vertebrate Limb Regeneration,” Wiley, New York. 3. Brockes, J. P. (1997). Amphibian limb regeneration: Rebuilding a complex structure. Science 276, 81– 87. 4. Echeverri, K., Clarke, J. D., and Tanaka, E. M. (2001). In vivo imaging indicates muscle fiber dedifferentiation is a major contributor to the regenerating tail blastema. Dev. Biol. 236, 151– 164. 5. Hay, E. D. (1959). Electron microscopic observations of muscle dedifferentiation in regenerating Amblystoma limbs. Dev. Biol. 1, 555–585. 6. 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