Disruption of actin cytoskeleton and anchorage-dependent cell spreading induces apoptotic death of mouse neural crest cells cultured in vitro.код для вставкиСкачать
THE ANATOMICAL RECORD PART A 282A:130 –137 (2005) Disruption of Actin Cytoskeleton and Anchorage-Dependent Cell Spreading Induces Apoptotic Death of Mouse Neural Crest Cells Cultured In Vitro ATSUSHI HINOUE,1,2 TOSHIYA TAKIGAWA,1 TAKASHI MIURA,1 YOSHIHIKO NISHIMURA,2 SHIGEHIKO SUZUKI,2 AND KOHEI SHIOTA1,3* 1 Department of Anatomy and Developmental Biology, Kyoto University Graduate School of Medicine, Kyoto, Japan 2 Department of Plastic and Reconstructive Surgery, Kyoto University Graduate School of Medicine, Kyoto, Japan 3 Congenital Anomaly Research Center, Kyoto University Graduate School of Medicine, Kyoto, Japan ABSTRACT In vertebrate embryos, neural crest cells emigrate out of the neural tube and contribute to the formation of a variety of neural and nonneural tissues. Some neural crest cells undergo apoptotic death during migration, but its biological signiﬁcance and the underlying mechanism are not well understood. We carried out an in vitro study to examine how the morphology and survival of cranial neural crest (CNC) cells of the mouse embryo are affected when their actin cytoskeleton or anchorage-dependent cell spreading is perturbed. Disruption of actin ﬁber organization by cytochalasin D (1 g/ml) and inhibition of cell attachment by matrix metalloproteinase-2 (MMP-2; 2.0 units/ml) were followed by morphologic changes and apoptotic death of cultured CNC cells. When the actin cytoskeleton was disrupted by cytochalasin D, the morphologic changes of cultured CNC cells preceded DNA fragmentation. These results indicate that the maintenance of cytoskeleton and anchorage-dependent cell spreading are required for survival of CNC cells. The spatially and temporally regulated expression of proteinases may be essential for the differentiation and migration of neural crest cells. © 2005 Wiley-Liss, Inc. Key words: cranial neural crest; apoptotic cell death; anoikis; actin cytoskeleton; anchorage dependency; mouse embryo During the development of vertebrate embryos, neural crest cells develop at the junction between the neural plate and the surface ectoderm. They migrate along spatially and temporally distinct pathways and differentiate into a variety of neuronal and nonneuronal cell types that are important in the formation of craniofacial structures, the cardiovascular system, and much of the peripheral nervous system (Le Douarin and Kalcheim, 1999). It has been shown that some cells in the cranial and trunk neural crests die by apoptosis during migration and that such cell death may play crucial roles in differentiation and migration of neural crest cells (Jeffs and Osmond, 1992; Jeffs et al., 1992; Hirata and Hall, 2000). Jeffs et al. (1992) observed cell death in speciﬁc populations of cranial neural crest (CNC) cells and postulated that it may contribute © 2005 WILEY-LISS, INC. to the patterning of early CNC migration. In the trunk of embryos, Wakamatsu et al. (1998) demonstrated that Grant sponsor: the Japanese Ministry of Education, Culture, Sports, Science and Technology; Grant number: 12670016 and 13470003. *Correspondence to: Kohei Shiota, Department of Anatomy and Developmental Biology, Kyoto University Graduate School of Medicine, Kyoto 606-8501, Japan. Fax: 81-75-751-7529. E-mail: firstname.lastname@example.org Received 21 June 2004; Accepted 20 October 2004 DOI 10.1002/ar.a.20150 Published online 2 January 2005 in Wiley InterScience (www.interscience.wiley.com). NEURAL CREST CELL APOPTOSIS some neural crest cells undergo apoptosis on the lateral migration pathway, and they argued that such cell death may help neural crest cells ﬁnd the right migration pathway and remove “ectopic” cells by a “proofreading mechanism.” They suggested that some environmental cues regulate the survival and death of neural crest cells. Developmental neuronal cell death has been reported to occur in both the central and peripheral nervous systems and is assumed to contribute to eliminating excessive and inappropriately located cells (Jacobson, 1991; Wakamatsu et al., 1998; Maynard et al., 2000). Various mechanisms have been proposed for developmental neuronal death, and it seems that the mechanism of cell death is not the same at different locations and at various stages in development. Since apoptotic death of neural crest cells often occurs after they leave the neural tube and become nonepithelial, we postulated that the survival of neural crest cells may depend on anchorage-dependent cell spreading and the maintenance of normal cytoarchitecture. Such anchorage-dependent survival has been noted in some epithelial cell types (Boudreau et al., 1995a, 1995b) but has not been demonstrated so far in neural crest cells. To investigate whether anchorage-dependent cell spreading and maintenance of cytoarchitecture are required for survival of CNC cells, we undertook an in vitro study where their actin cytoskeleton and attachment to the substratum were disrupted by chemical agents. Cultured CNC cells emigrating out of the explanted mouse embryonic neural tube were treated with cytochalasin D and matrix metalloproteinase-2 (MMP-2) to disrupt their actin cytoskeleton and adhesion to the underlying substratum, respectively. Cytochalasin D blocks the formation of microﬁlament structures by abrogating actin polymerization and cytochalasin D-treated cells cannot maintain normal morphology (Korn, 1982). MMP-2 degrades extracellular matrix (ECM) components such as type IV and V collagens, laminin-5, elastin, ﬁbronectin, and proteoglycans, thereby disrupting cell-ECM interactions (Okada et al., 1990; Giannelli et al., 1997; Zuo et al., 1998). It has been shown that MMP-2 has an important functional role in epithelial-mesenchymal transformation (EMT) and migration of neural crest cells and that perturbation of MMP activity may lead to neural crest-related congenital defects (Cai et al., 2000; Cai and Brauer, 2002; Duong and Erickson, 2004). We analyzed the effects of cytochlasin D and MMP-2 on the morphology and survival of cultured CNC cells by cytochemical staining for actin microﬁlaments and by in situ labeling of DNA fragmentation (TUNEL method). The disruption of actin ﬁber organization and adhesion to the substratum was followed by apoptotic death of cultured CNC cells, suggesting that properly organized cytoarchitecture and anchorage-dependent cell spreading are essential for survival of CNC cells. MATERIALS AND METHODS Animals ICR strain mice (SLC Japan, Shizuoka, Japan) were maintained in a temperature- and humidity-controlled animal facility with a 12-hr light/12-hr dark cycle. Animals were given laboratory chow and tap water ad libitum. Virgin female mice were mated overnight with a male mouse, and the noon of the day on which a vaginal plug was found was taken as embryonic day 0.5 (E0.5). On E8.5, embryos were obtained by Caesarean section and 131 transferred to sterile Tyrode buffer solution. The experimental protocol was approved by the Committee for Animal Experimentation of Kyoto University Graduate School of Medicine. Neural Crest Cell Explant Culture Primary culture of mouse CNC cells was carried out according to the method originally described by Ito and Takeuchi (1984) and Murphy et al. (1991). Each mouse embryo (E8.5) was treated with 0.25% trypsin/PBS for 15 min and the hindbrain neural folds were isolated. The dorsal ridge of the neural folds was surgically removed free from the surrounding tissues and cultured on a 35 mm culture dish coated with ﬁbronectin (Becton Dickinson). The culture medium contained 90% ␣-MEM medium (Gibco-BRL), 10% fetal bovine serum (Gibco-BRL), 4% chick embryo extract (Gibco-BRL), 50 U/ml penicillin, 50 g/ml streptomycin (Gibco-BRL), and 1% insulin-transferrin-selenium-X (Gibco-BRL). The cultures were maintained for 48 hr at 37°C in a CO2 incubator under a humidiﬁed atmosphere composed of 95% air and 5% CO2. At 48 hr after culture, the neural folds in the colonies were scraped away with syringe needles, and the remaining CNC cells, which had migrated out of the neuroepithelium, were used for the following experiments. Cranial neural crest cells were identiﬁed by immunohistochemical staining with a rat antimouse monoclonal antibody 4E9R (Kubota et al., 1996), which was kindly provided by Dr. Kazuo Ito (Osaka University Graduate School of Science, Toyonaka, Japan). The 4E9R antibody has been shown to identify migratory mouse neural crest cells (Kubota et al., 1996). Treatment With Cytochalasin D and MMP-2 After preparation of cultured CNC cells as described above, the culture medium was replaced by a serum-free medium to eliminate the inﬂuence of substances contained in fetal bovine serum. Then, either cytochalasin D (1 g/ml; Sigma, St. Louis, MO) or MMP-2 (2.0 unit/ml; Cosmo Bio, Tokyo, Japan) was added to the medium for experimental groups. For stock solutions, cytochalasin D and MMP-2 were dissolved in DMSO and PBS, respectively. The ﬁnal concentration of cytochalasin-D (1 g/ml) was determined according to previous studies in which microtubule assembly and cell shape of cultured cells were disrupted (Nishi et al., 2002; Nemeth et al., 2004). The concentration of MMP-2 (2.0 unit/ml) was used because the concentration 1.0 unit/ml or below had no observable effects on cultured CNC cells. In control groups, an equivalent volume of the vehicle was added to the culture medium. After adding the chemicals, each culture dish was further incubated in a CO2 incubator and was observed and photographed at every hour using a Nikon Diaphoto phase-contrast microscope (Nikon, Tokyo, Japan). At 12 hr after treatment, cells in culture dishes were ﬁxed with 4% paraformaldehyde for further stainings and the TUNEL reaction. Dual Staining for Actin Fibers and Nuclear DNA The ﬁxed CNC cells were washed three times with PBS, immersed in 0.1% Triton X-100/PBS, then incubated for 10 min at room temperature with 33 M phalloidin- 132 HINOUE ET AL. rhodamin (Sigma) and 0.025% Hoechst33342 (Sigma) dissolved in PBS. After incubation, the cells in the dishes were washed three times with PBS and coverslipped. The cells were observed using an Axioplan 2 ﬂuorescence microscope (Carl Zeiss, Germany) equipped with ﬂuorescein ﬁlters and were photographed using a CoolSNAP CCD camera (Photometrics). In Situ Labeling of DNA Fragmentation by TUNEL Method The in situ visualization technique for DNA fragmentation was carried out according to the TUNEL method (Gavrieli et al., 1992; Mori et al., 1995). Fixed CNC cells were washed three times with double-distilled water, airdried, and treated with 5 g/ml proteinase K (Wako Pure Chemical, Tokyo, Japan). After proteinase K treatment, the cells were incubated in TdT buffer containing 12.5 M biotinylated-dUTP (Boehringer Mannheim) and 0.15 unit/l TdT (Takara, Kyoto, Japan) at 37°C for 70 min. Then, they were reacted with rhodamine-avidin (Sigma) for visualization of fragmented DNA. After being rinsed several times with PBS, the samples were coverslipped and observed. The samples were photographed using a Zeiss Axioplan 2 ﬂuorescence microscope and a CoolSNAP CCD camera (Photometrics). For each sample, the ratio of TUNEL-positive cells to the total cells was calculated. Cell counts were executed on the monitor of a Power Macintosh computer (Apple) using a counting tool of the National Institutes of Health Image program (http://rsb.info. nih.gov/nih-image). RESULTS Morphologic Changes of Cultured CNC Cells Treated With Cytochalasin D and MMP-2 In control cultures, numerous cells began to emigrate out of the explanted neural tube within 4 hr after culture and their emigration and mitotic divisions continued for over 72 hr. Migrating cells at the peripheral part of the colonies showed the bipolar or multipolar morphology, which is typical for neural crest cells, as has been described by Ito and Takeuchi (1984) (Fig. 1A). Immunohistochemical staining with a monoclonal antibody against neural crest cells (4E9R) (Kubota et al., 1996) revealed that over 90% of the cells emigrating out of the explanted neural tube were 4E9R-positive, indicating that they were CNC cells (Fig. 1B). By 60 hr in culture, many of those emigrated cells began to extend axon-like protrusions and appeared to undergo morphologic differentiation (data not shown). Therefore, the cells cultured for 48 hr were used for the following experiments. When CNC cells were cultured with cytochalasin D (1 g/ml), obvious morphologic changes were observed within 1 hr. Many cells showed a blebbing appearance, which is characteristic to apoptotic cells. By 12 hr after culture, the cells retracted their cell protrusions (ﬁlopodia) and became shrunken and rounded (Fig. 1C). When MMP-2 (2.0 units/ml) was added to the culture medium, cultured cells showed morphologic changes such as membrane blebbing and retraction of ﬁlopodia, and the cell area was reduced as compared with controls (Fig. 1D). Some cells became rounded. Morphologic Changes of Nucleus and Actin Fiber Organization of Cultured CNC Cells When the cells in control cultures were subjected to dual staining for actin ﬁbers and nuclear DNA, the morphology of cell nuclei and the arrangement of actin stress ﬁbers in the cytoplasm appeared normal (Fig. 2A and B). Actin ﬁbers were well organized and arranged orderly in their cytoplasm. The cells were spread well and had numerous ﬁlopodia. When the cultured CNC cells were treated with cytochalasin D, they became remarkably shrunken within 1 hr and their actin ﬁbers became disorganized and condensed around nuclei (Fig. 2C). Most of the cells showed nuclear shrinkage and chromatin condensation (Fig. 2D), which are often observed in apoptotic cells. When cultured cells were treated with MMP-2, many of the cells appeared to retract ﬁlopodia and the cell area was reduced by 12 hr after treatment, indicating that the cell-matrix attachment was disrupted to some extent (Fig. 2E). Some cells with cytoplasmic shrinkage were associated with actin ﬁber condensation around the nuclei, and condensed nuclei were intensely stained with Hoechst 33342, indicative of possible apoptotic bodies (Fig. 2F). Apototic Death of Cultured CNC Cells In each culture, apoptotic cells were identiﬁed by the TUNEL method, which detects DNA fragmentation, and the number of TUNEL-positive cells was counted. TUNEL-positive cells often had condensed nuclei and small apoptotic bodies (Fig. 3A–C). The ratio of TUNELpositive cells to the total number of cells was calculated by counting at least 200 cells in each culture and the data were compared between the groups (n ⫽ 5 for each group). The frequencies of apoptotic CNC cells in cultures treated with cytochalasin D and MMP-2 were 13.4% ⫾ 2.0% (mean ⫾ SE) and 20.1% ⫾ 2.0%, respectively, which were signiﬁcantly higher than the control value (5.4%% ⫾ 0.5%; Fig. 3C). The frequency of apoptotic cells was higher in the MMP-2-treated group than in the cytochalasin D-treated group, although the morphologic change was less severe in the former group (Figs. 1 and 2). DISCUSSION By using in vitro culture of migrating CNC cells, we have demonstrated that the survival of CNC cells is dependent on their cytoarchitecture maintained by actin stress ﬁbers as well as on anchorage-dependent cell spreading. When the intercellular actin ﬁber organization of cultured CNC cells was disrupted by cytochalasin D, they rapidly became rounded and underwent apoptotic morphologic changes. It is interesting to note that the dying cells showed such morphologic alterations before they became TUNEL-positive. Since cytochalasin D abrogates actin polymerizaion and disrupts actin ﬁlaments (Walling et al., 1988), it is likely that malfunction of actin ﬁbers and/or disruption of normal cytoarchitecture can induce cell death without directly affecting nuclear DNA. Although DNA fragmentation is a major molecular landmark of apoptotic cell death, it has been shown that apoptosis is a process involving some cytoplasmic alterations and does not necessarily require nuclear DNA fragmentation or other changes in the nucleus at its initial step (Cohen et al., 1992; Falcieri et al., 1993; Oberhammer et al., 1993). It has been well accepted that the maintenance NEURAL CREST CELL APOPTOSIS 133 Fig. 1. Cultured CNC cells in the control and experimental groups. A: A phase-contrast image of CNC cells in the control group cultured for 48 hr. The cells are spread well and have numerous ﬁlopodia. B: Immunohistochemical staining of a control culture with the 4E9R monoclonal antibody, which identiﬁes neural crest cells. Most of the cells are 4E9Rpositive (green). Nuclei are stained with Hoechst 33342 (purple). C: CNC cells cultured for 12 hr with cytochalasin D (1 g/ml). Most of the cells are shrunk and rounded and have retracted ﬁlopodia. D: CNC cells cultured for 12 hr with MMP-2 (2.0 unit/ml). Some cells show membrane blebbing and have retracted cell protrusions (arrowheads). The cell area is reduced as compared with that in controls (A). Scale bar ⫽ 100 m. of cell morphology and differentiation is dependent on the actin cytoskeleton (Hay, 1993). In addition, recent studies suggest that the cytoskeleton and cortical actin network play critical roles in various intercellular signaling (Aplin and Juliano, 1999; Zoubiane et al., 2004). Therefore, disruption of the actin cytoskeleton by cytochalasin D may not only have affected the cytoarchitecture but also have precluded effective signaling via the cytoskeleton, resulting in cell death. MMP-2 degrades various ECM proteins including ﬁbronectin, type IV and V collagens, laminin, and elastin (Vassalli and Pepper, 1994; Werb and Chin, 1998). Recently, Duong and Erickson (2004) demonstrated that MMP-2 is expressed as neural crest cells detach from the 134 HINOUE ET AL. Fig. 2. Dual staining for actin ﬁbers (red) and nuclear DNA (blue; A, C, and E) and nuclear staining with Hoechst 33342 in the same ﬁelds (B, D, and F). A and B: CNC cells in a control culture. The arrangement of actin ﬁbers is well organized (A) and their nuclei are round and appear healthy (B). C and D: CNC cells at 12 hr after cytochalasin D treatment. Actin ﬁbers aggregate around nuclei (C), and nuclei are clearly condensed (D). E and F: CNC cells at 12 hr after MMP-2 treatment. Cells are not so well expanded as in the control culture (A), and actin ﬁbers are not well organized and appear aggregated around nuclei in some cells (stained heavily in red; E). Condensation of nuclear chromatin is recognized (arrowheads in F). Scale bar ⫽ 100 m. NEURAL CREST CELL APOPTOSIS Fig. 3. Apoptotic cell death of cultured CNC cells visualized by the TUNEL method. A: Control culture. B: Cells treated with cytochalasin D for 12 hr. C: Cells treated with MMP-2 for 12 hr. TUNEL-positive nuclei and apoptotic bodies are visualized in orange yellow. Scale bar ⫽ 100 m. D: The frequency of TUNEL-positive cells in cultured CNC cells. The percentage of TUNEL-positive cells increased signiﬁcantly in both treated groups as compared with controls (asterisk, P ⬍ 0.05; double asterisk, P ⬍ 0.01 vs. control). Error bars show SEM (n ⫽ 5). neural epithelium during EMT but is rapidly extinguished as they disperse. They also showed that MMP inhibitors and knockdown of MMP-2 expression perturb EMT that generates neural crest cells but do not affect migration of neural crest cells, suggesting that MMP-2 plays a crucial role at some steps in EMT of neural crest cells but is not required for the later migration process. Cai et al. (2000) observed the expression of MMP-2 mRNA in the craniofacial region of avian embryos and found that early migrating CNC cells do not synthesize MMP-2 mRNA but can interact with extracellular MMP-2 protein synthesized by the mesoderm. Furthermore, Cai and Brauer (2002) showed that neural crest migration is decreased when the MMP activity is perturbed. Thus, it seems that proteolytic degradation of ECM by MMP-2 is required at some stages of neural crest development but its expression may be ﬁnely regulated spatially and temporally so that the differentiation and migration of neural crest cells can take place properly. Patch mutant mice, which have a deﬁcit in MMP-2 and membrane-type MMP expression and decreased migratory capacity of craniofacial mesenchyme (Robbins et al., 1999), exhibit neural crest-related craniofacial and cardiac defects (Morrison-Graham et al., 1992; Schatteman et al., 1995). 135 We showed in the present study that treatment of cultured CNC cells with MMP-2 disrupts cell-matrix interaction and induces apoptotic death. When treated continuously with MMP-2, cultured CNC cells retracted their protrusions (ﬁlopodia) and appeared to detach from the substratum, increasing TUNEL-positive cells by 12 hr. Thus, adhesion of CNC cells to ECM seems essential not only for maintaining their normal cell shape but also for their survival. This ﬁnding is consistent with the previous ﬁnding that some epithelial cells undergo apoptosis when they are separated from the basement membrane (Schmidt et al., 1993; Frisch and Francis, 1994). We have conﬁrmed that degradation of ECM components by MMP-1 (type I collagenase) also resulted in apoptotic death of cultured mouse CNC cells (data not shown). In the present study, it was noted that the proportion of TUNEL-positive cells, which is indicative of DNA fragmentation, was higher in MMP-2-treated cells than in cytochalasin D-treated cells, although the morphologic effect appeared more severe in the latter (Figs. 2 and 3). When the CNC cells were treated with 1 g/ml cytochalasin D, many cells became rounded and their nuclei appeared condensed. However, their nuclei became rodlike (Fig. 2D), which were different from typically pycnotic nuclei, as were seen in MMP-2-treated cells (Fig. 2F). Thus, actin ﬁber disorganization induced by cytochalasin D may not instantly result in apoptotic death of CNC cells. It has been reported that various types of epithelial cells need anchorage-dependent cell spreading for survival and that they undergo apoptotic death when their cell-matrix attachment is disrupted (Boudreau et al., 1995a, 1995b; Roberts et al., 2002). Frisch and Francis (1994) coined the term “anoikis” for such a kind of apoptotic cell death. It is likely that adhesion-dependent regulation of cell survival is mediated by integrin signaling and that efﬁcient cellECM adhesion is required for forming focal adhesion plaques by clustering ECM-receptor integrins. It has been shown that some signaling pathways of tyrosine phosphorylation mediated by focal adhesion kinase (FAK) are required for organization and maintenance of actin stress ﬁbers to assemble cytoskeleton-associated proteins, such as paxillin, vinculin, talin, tenascin, and ␣-actinin, at the cytoplasmic domains of integrins (Clark and Brugge, 1995; Miyamoto et al., 1995). Frisch et al. (1996) showed that the interaction of integrins with ECM proteins can activate FAK and thereby suppress apoptosis in endothelial and other epithelial cells. In the case of endothelial cells, not only cell-ECM adhesion but also cell spreading are important for preventing them from entering the process of apoptosis. Re et al. (1994) demonstrated that endothelial cells cultured under low concentrations of ﬁbronectin or vitronectin became rounded and underwent rapid cell death, while the cells became ﬂattened and remained viable under high substrate concentrations. They concluded that cell-matrix attachment is not sufﬁcient for sustaining cell viability but cells need to achieve some shape changes to survive. Chen et al. (1997) directly examined the effects of cell spreading on growth and viability and showed that growth and survival of cultured endothelial cells increased as the extent of cell spreading increased but were independent of the total area of cell-ECM contact. Furthermore, it was shown that DNA synthesis is tightly coupled with the cell shape (Folkman and Moscona, 1978) and that stretch stimuli activate DNA synthesis and cell proliferation (Lansman et 136 HINOUE ET AL. al., 1987; Olesen et al., 1988). These results support the hypothesis that unfavorable alterations of cell architecture and cell spreading can affect the survival and differentiation of some cells and trigger their apoptosis. During the migration of neural crest cells, their interaction with ECM may be crucial. It is likely that some proteinases including MMPs synthesized by mesenchymal cells help the EMT and migration of neural crest cells but their expression needs to be temporally and spatially regulated not only to facilitate their differentiation but also to keep them viable. Recent molecular studies have demonstrated that a cystein protease family caspase, which is an ICE/CED-3 gene product, is involved in the onset of apoptosis (Miura et al., 1993; Nicholson et al., 1995; Kuida et al., 1996; Mashima et al., 1997; Miller, 1997). Caspase-1 (ICE) and caspase-3 (CPP-32), which cleave the existing actin ﬁbers as a substrate, are activated following the disruption of cell-ECM adhesion (Boudreau et al., 1995b; Mashima et al., 1997). Actin is an inhibitor of deoxyribonuclease I (DNase I), which is a candidate endonuclease responsible for apoptotic DNA fragmentation (Peitsch et al., 1993), and the actin cleaved by ICE/CPP-32 loses the ability to inhibit DNase I (Kayalar et al., 1996). These data are consistent with the assumption that the disruption of actin ﬁber organization is a critical event for commencement of apoptosis. It is possible that the perturbation of actin microﬁlaments and the disruption of cell adhesion to ECM or adjacent cells can induce cell shape changes and perturb some signaling pathways in the cell. As for the roles of caspases in developmental apoptosis, Umpierre et al. (2001) demonstrated that activated caspase-3 and DNA fragmentation were colocalized in the mesenchymal cells of branchial arches and in neuroepithelial cells of day 9 mouse embryos. The cells expressing caspase-3 were found to be abundant in the mesenchyme of the ﬁrst and second branchial arches, which coincided with the CNC cell migratory areas in E8.5 mouse embryos (Kubota et al., 1996). It was also shown that caspase-3deﬁcient mice exhibit embryonic or early postnatal lethality and their central nervous system development was severely impaired (Kuida et al., 1996). Further, caspase-3 deﬁciency in mice resulted in decreased embryonic neuroblast apoptosis and neoplastic growth of the brain (Pompeiano et al., 2000). Thus, caspase-3 seems to play a critical role in the induction of morphogenetic apoptosis in embryos, especially in the nervous system. These reports warrant further investigation for elucidating the mechanisms of differentiation and migration of CNC cells as well as the signiﬁcance of their apoptotic death observed in craniofacial morphogenesis. ACKNOWLEDGMENTS The authors are grateful to Dr. Kazuo Ito, Osaka University Graduate School of Science, for providing the 4E9R antibody and Dr. Shigehito Yamada for his technical assistance. LITERATURE CITED Aplin AE, Juliano RL. 1999. Integrin and cytoskeletal regulation of growth factor signaling to the MAP kinase pathway. J Cell Sci 112:695–706. Boudreau N, Myers C, Bissell MJ. 1995a. From laminin to lamin: regulation of tissue-speciﬁc gene expression by the ECM. Trends Cell Biol 5:1– 4. Boudreau N, Sympson C J, Werb Z, Bissell M. 1995b. Suppression of ICE and apoptosis in mammary epithelial cells by extracellular matrix. Science 267:891– 893. Cai DH, Vollber TM Sr, Hahn-Dantona E, Quigley JP, Brauser PR. 2000. MMP-2 expression during early avian cardiac and neural crest morphogenesis. Anat Rec 259:168 –179. Cai DH, Brauer PR. 2002. Synthetic matrix metalloproteinase inhibitor decreases early cardiac neural crest migration in chicken embryos. Dev Dyn 224:441– 449. Chen CS, Mrksich M, Huang S, Whitesides GM, Ingber DE. 1997. Geometric control of cell life and death. Science 276:1425–1428. Clark EA, Brugge JS. 1995. Integrins and signal transduction pathways: the road taken. Science 268:233–239. Cohen GM, Sun X-M, Snowden T, Dinsdale D, Skiletter DN. 1992. Key morphological features of apoptosis may occur in the absence of internucleosomal DNA fragmentation. Biochem J 286:331–334. Duong T, Erickson CA. 2004. MMP-2 plays an essential role in producing epithelial-mesenchymal transformations in the avian embryo. Dev Dyn 229:42–53. Falcieri E, Mrtelli AM, Bareggi R, Catal di A, Cocco L. 1993. The protein kinase inhibitor staurosporine induces morphological changes typical of apoptosis in MOLT-4 cells without concomitant DNA fragmentation. Biochem Biophys Res Commun 193:19 –25. Folkman J, Moscona A. 1978. Role of cell shape in growth control. Nature 273:345–349. Frisch SM, Francis H. 1994. Disruption of epithelial cell-matrix interactions induces apoptosis. J Cell Biol 124:619 – 626. Frisch SM, Buori K, Ruoslahti E, Chan-Hui PY. 1996. Control of adhesion-dependent cell survival by focal adhesion kinase. J Cell Biol 134:793–799. Gavrieli Y, Sherman Y, Ben-Sasson SA. 1992. Identiﬁcation of programmed cell death in situ via speciﬁc labeling of nuclear DNA fragmentation. J Cell Biol 119:493–501. Giannelli G, Falk-Marzillier J, Schiraldi O, Stetler-Stevenson WG, Quaranta V. 1997. Induction of cell migration by matrix metalloprotease-2 cleavage of laminin-5. Science 277:225–228. Hay ED. 1993. Extracellular matrix alters epithelial differentiation. Curr Opin Cell Biol 5:1029 –1035. Hirata M, Hall BK. 2000. Temporospatial patterns of apoptosis in chick embryos during the morphogenetic period of development. Int J Dev Biol 44:757–768. Ito K, Takeuchi T. 1984. The differentiation in vitro of the neural crest cells of the mouse embryos. J Embryol Exp Morphol 84:49 – 62. Jacobson M. 1991. Developmental neurobiology, 3rd ed. New York: Plenum Press. Jeffs P, Osmond M. 1992. Asegmented pattern of cell death during development of the chick embryo. Anat Embryol (Berl) 185:589 – 598. Jeffs P, Jaques K, Osmond M. 1992. Cell death in cranial neural crest development. Anat Embryol (Berl) 85:583–588. Kayalar C, Örd T, Testa MP, Zhong L-T, Bredesen DE. 1996. Cleavage of actin by interleukin 1␤-converting enzyme to reverse DNase I inhibition. Proc Natl Acad USA 93:2234 –2238. Korn ED. 1982. Actin polymerization and its regulation by proteins from nonmuscle cells. Physiol Rev 62:1519 –1530. Kubota Y, Morita T, Ito K. 1996. New monoclonal antibody (4E9R) identiﬁes mouse neural crest cells. Dev Dyn 206:368 –378. Kuida K, Zheng TS, Na S, Kuan C, Yang D, Krasuyama H, Rakic P, Flavell RA. 1996. Decreased apoptosis in the brain and premature lethality in CPP32-deﬁcient mice. Nature 384:368 –372. Lansman JB, Hallam TJ, Rink TJ. 1987. Single stretch-activated ion channels in vascular endothelial cells as mechanotransducers? Nature 325:811– 813. Le Douarin NM, Kalcheim C. 1999. The neural crest. New York: Cambridge University Press. Mashima T, Naito M, Noguchi K, Miller DK, Nicholson DW, Tsuruo T. 1997. Actin cleavage by CPP-32/apopain during the development of apoptosis. Oncogene 14:1007–1012. Maynard TM, Wakamatsu Y, Weston JA. 2000. Cell interactions within nascent neural crest cell populations transiently promote death of neurogenic precursors. Development 127:4561– 4572. NEURAL CREST CELL APOPTOSIS Miller DK. 1997. The role of the caspasecfamily of cysteine proteases in apoptosis. Semin Immunol 9:35– 49. Miura M, Zhu H, Rotello R, Hartwieg EA, Juan J. 1993. Induction of apoptosis in ﬁbroblasts by IL-1 beta-converting enzyme, a mammalian homolog of the C. elegans cell death gene ced-3. Cell 75:653– 660. Miyamoto S, Teramoto H, Coso OA, Gutkind JS, Brubelo PD, Akiyama SK. 1995. Integrin function: molecular hierarchies of cytoskeletal and singaling molecules. J Cell Biol 131:791– 805. Mori C, Nakamura N, Kimura S, Irie H, Takigawa T, Shiota K. 1995. Programmed cell death in the interdigital tissue of the fetal mouse limb is apoptosis with DNA fragmentation. Anat Rec 242:103–110. Morrison-Graham K, Schatteman GC, Bork T, Bowen-Pope DF, Weston JA. 1992. A PDGF receptor mutation in the mouse (Patch) perturbs the development of a non-neuronal subset of neural crestderived cells. Development 115:133–142. Murphy M, Bernard O, Reid K, Bartlett PF. 1991. Cell lines derived from mouse neural crest are representative of cells at various stages of differentiation. J Neurobiol 22:522–535. Nemeth ZH, Deitch EA, Davidson MT, Szabo C, Vizi ES, Hasko G. 2004. Disruption of the actin cytoskeleton results in nuclear factor-kB activation and inﬂammatory mediator production in cultured human intestinal epithelial cells. J Cell Physiol 200:71– 81. Nicholson DW, Ali A, Thornberry NA, Vailliancourt JP, Ding CK, Gallant M, Grifﬁn PR, Labelle M, Lazebnik YA, Munday NA, Yu VL, Miller DK. 1995. Identiﬁcation and inhibition of the ICE/CED-3 protease necessary for mammalian apoptosis. Nature 376:37– 43. Nishi K, Schnier JB, Bradbury EM. 2002. Cell shape change precedes staurosporine-induced stabilization and accumulation of p27kip1. Exp Cell Res 280:233–243. Oberhammer F, Wilson JW, Dive C, Morris ID, Hickman JA, Wakeling AE, Walker PR, Sikorska M. 1993. Apoptotic death in epithelial cells: cleavage of DNA to 300 and/or 50 kb fragments prior to or in the absence of internucleosomal fragmentation. EMBO J 12:3697– 3688. Okada Y, Morodomi T, Enghild JJ, Suzuki K, Yasui A, Nakanishi I, Salvesen G, Nagase H. 1990. Matrix metalloproteinase 2 from human rheumatoid synovial ﬁbroblasts: puriﬁcation and activation of the precursor and enzymic properties. Eur J Biochem 194:721–730. Olesen SP, Clapham DE, Davies PF. 1988. Haemodynamic shear stress activates a K⫹ current in vascular endothelial cells. Nature 331:168 –170. Peitsch MC, Polzar B, Stephan H, Crompton T, MacDonald HR, Mannherz HG, Tschopp J. 1993. Characterization of the endoge- 137 nous deoxyribonuclease involved in nuclear DNA degradation during apoptosis (programmed cell death). EMBO J 12:371–377. Pompeiano M, Blaschle AJ, Flavell RA, Srinivasan A, Chun J. 2000. Decreased apoptosis in proliferative and postmitotic regions of the Caspase 3-deﬁcient embryonic central nervous system. J Comp Neurol 423:1–12. Re F, Zanetti A, Sironi M, Polentarutti N, Lanfrancone L, Dejana E, Colotta F. 1994. Inhibition of anchorage-dependent cell spreading triggers apoptosis in cultured human endothelial cells. J Cell Biol 127:537–546. Robbins JR, McGuire PG, Wehrle-Haller B, Rogers SL. 1999. Diminished matrix metalloproteinase 2 (MMP-2) in ectomesenchyme-derived tissues of the Patch mutant mouse: regulation of MMP-2 by PDGF and effects on mesencymal cell migration. Dev Biol 212:255– 263. Schatteman GC, Motley ST, Effmann EL, Bowen-Pope DF. 1995. Platelet-derived growth factor receptor alpha subunit deleted Patch mouse exhibits severe cardiovascular dysmorphogenesis. Teratology 51:351–366. Schmidt JW, Piepenhagen PA, Nelson WJ. 1993. Modulation of epithelial morphogenesis and cell fate by cell-to-cell signals and regulated cell adhesion. Semin Cell Biol 4:161–173. Umpierre CC, Little SA, Mirkes PE. 2001. Co-localization of active caspase-3 and DNA fragmentation (TUNEL) in normal and hyperthermia-induced abnormal mouse development. Teratology 63:134 – 143. Vassalli JD, Pepper MS. 1994. Tumour biology: membrane proteases in focus. Nature 370:14 –15. Wakamatsu Y, Mochii M, Vogel KS, Weston JA. 1998. Avian neural crest-derived neurogenic precursors undergo apoptosis on the lateral migration pathway. Development 125:4205– 4213. Walling EA, Krafft GA, Ware BR. 1988. Actin assembly activity of cytochalasins and cytochalasin analogs assayed using ﬂuorescence photobleaching recovery. Arch Biochem Biophys 264:321–332. Werb Z, Chin JR. 1998. Extracellular matrix remodeling during morphogenesis. Ann NY Acad Sci 857:110 –118. Zoubiane GS, Valentijn A, Lowe ET, Akhtar N, Bagley S, Gilmore AP, Streuli CH. 2004 A role for the cytoskeleton in prolactin-dependent mammary epithelial cell differentiation. J Cell Sci 117(Pt 2):271– 280. Zuo J, Ferguson TA, Hernandez YJ, Stetler-Stevenson WG, Muir D. 1998. Neuronal matrix metalloproteinase-2 degrades and inactivates a neurite-inhibiting chondroitin sulfate proteoglycan. J Neurosci 18:5203–5211.