Search tips
Search criteria 


Logo of plosonePLoS OneView this ArticleSubmit to PLoSGet E-mail AlertsContact UsPublic Library of Science (PLoS)
PLoS One. 2010; 5(8): e12369.
Published online 2010 August 24. doi:  10.1371/journal.pone.0012369
PMCID: PMC2927436

Dcas Supports Cell Polarization and Cell-Cell Adhesion Complexes in Development

Madhuri Kango-Singh, Editor


Mammalian Cas proteins regulate cell migration, division and survival, and are often deregulated in cancer. However, the presence of four paralogous Cas family members in mammals (BCAR1/p130Cas, EFS/Sin1, NEDD9/HEF1/Cas-L, and CASS4/HEPL) has limited their analysis in development. We deleted the single Drosophila Cas gene, Dcas, to probe the developmental function of Dcas. Loss of Dcas had limited effect on embryonal development. However, we found that Dcas is an important modulator of the severity of the developmental phenotypes of mutations affecting integrins (If and mew) and their downstream effectors Fak56D or Src42A. Strikingly, embryonic lethal Fak56D-Dcas double mutant embryos had extensive cell polarity defects, including mislocalization and reduced expression of E-cadherin. Further genetic analysis established that loss of Dcas modified the embryonal lethal phenotypes of embryos with mutations in E-cadherin (Shg) or its signaling partners p120- and β-catenin (Arm). These results support an important role for Cas proteins in cell-cell adhesion signaling in development.


Cas proteins are non-catalytic scaffolding proteins that control signaling relevant to cell attachment, migration, cycle, and survival (reviewed in [1], [2], [3]). The four paralogous Cas family proteins in vertebrates include BCAR1/p130Cas [4], NEDD9/HEF1/Cas-L [5], EFS/Sin [6] and CASS4/HEPL [7], of which BCAR1 and NEDD9 have been the most intensively studied. The best established functional role for these proteins is at focal adhesions, where they interact with FAK and Src to transmit integrin-initiated signals from the extracellular matrix to downstream effectors, leading to reorganization of the actin cytoskeleton and changes in motility and invasion [8][15].

Overexpression of Cas proteins contributes to the development of human cancer (reviewed in [3], [16]). BCAR1 is required for Src-dependent cellular transformation of murine fibroblasts [17], and conserves with NEDD9 the ability to enhance the production of matrix metalloproteases [18], enhancing tumor cell invasion of the extracellular matrix (ECM) [19], promoting mammary tumorigenesis and lung metastasis in MMTV-HER2 and other mouse models of cancer [19], [20]. NEDD9 has been defined as a component of an intracellular signaling switch that is important for epithelial-mesenchymal transition (EMT), based on activation of its downstream effector Rac [21]. TGFβ promotes EMT during tumor cell invasion through the ECM, and tissue remodeling in development. In mammals, TGFβ regulates both transcription and proteasomal degradation of NEDD9 [22], [23]; conversely, BCAR1 and NEDD9 reciprocally bind and regulate the activity of a subset of TGFβ effectors [24], [25], [26]. BCAR1 overexpression may predict aggressive estrogen receptor-negative cancers [27], [28]. Overexpression of NEDD9 supports oncogenic signaling in malignancies of the hematopoietic system [13], [29][32], and has been linked to increased cellular invasive behavior in breast and colorectal cancer cell lines [18], [33], squamous cell carcinomas of the head and neck [34], and enhanced metastatic potential in glioblastomas [35], melanomas [12], and some lung cancers [36], and to cell migration and EMT induced by chemical carcinogens [37]. Conversely, a null NEDD9 genotype significantly increases the latency of tumor incidence in the MMTV-PyVmT mammary cancer model [38].

While studies of the Cas group have emphasized important roles in cancer and other pathogenic conditions, little is known of their roles in normal development. Knockout of BCAR1 in mice leads to an embryonal lethal phenotype at day 11.5–12.5, associated with marked systemic congestion and growth retardation, and disordering of actin-based structures in the heart [17]. In contrast, knockout of NEDD9 results in viable, fertile animals, with minor defects in immune system maturation [39]. The presence of 4 paralogous family members with overlapping expression profiles [7], together with the difficulty of performing detailed phenotypic analysis in early embryonal development, have made it difficult to establish the required functions of Cas proteins in mammalian development.

By contrast, there is only a single Cas family protein in Drosophila, Dcas (CG1212). Dcas is highly expressed in the embryonic nervous system at stage 16 [40], as well as in the ventral ectoderm and ventral nerve cord primordial at earlier developmental stages (stages 9–12 [41]). The importance of DCas in Drosophila has been unclear. One recent study used an existing allele with a P-element insertion in an intron within the Dcas coding region, and a deficiency mutation overlapping Dcas and 5 adjacent genes, to establish a modifier role for Dcas in axonal fasciculation and axon guidance [40], but did not address the question of any potential early embryonal phenotypes. Although the protein is highly conserved with mammalian family members (68% with NEDD9 and 70% with BCAR1 [40]), null mutations in Drosophila orthologs of some of the most important mammalian interactors of Cas proteins, such as FAK (Fak56) [42] produce limited phenotypes. In the present study, we have used a FRT-excision-based strategy to delete the Dcas locus. Upon identification of an embryonal lethal phenotype affecting 10% of maternal-zygotic null embryos, we subsequently extensively probed the genetic interactions of Dcas relevant to cell migration and EMT. This work indicated evolutionary conservation of core Cas family signaling involving FAK, Src, and integrins. Combination of mutations in Dcas and Fak56 perturbed localization of polarity markers, including particularly E-cadherin (Shotgun, Shg), implying that DCas might also interact with the E-cadherin-associated cell junctional proteins. Subsequent experiments directly testing this idea identified novel and potent genetic interactions between Dcas and the cell-cell adhesion proteins Shotgun, Armadillo and p120-catenin, influencing cell polarity. These findings inform the understanding of Cas protein action both in development and in cancer progression.


Generation and characterization of a Dcas null allele

To study Dcas function in Drosophila development, we used a modification of FRT-excision technology [43]. A FRT-containing P-element upstream of the Dcas gene was provided by a P-element located within 50 bp of the start of the Dcas open reading frame (ORF). A downstream transposon was provided by a Pbac located between the end of the Dcas coding sequences and the assigned start codon of the CG7049 ORF. Using this technique, we generated a precise excision of the complete Dcas ORF on chromosome 3 (Fig. 1A). The resulting allele, which we call Dcas1, contains a deletion spanning the first through final coding exons of the Dcas gene, but retains the Dcas promoter region and flanking genes, as confirmed by extensive quantitative PCR using probes directed against the DNA of Dcas and flanking genes (results not shown). Homozygous Dcas1/Dcas1 mutants produce fertile progeny and can be maintained as a stable Dcas null strain.

Figure 1
Generation of the Dcas1 mutant stock.

To exclude the possiblity of secondary mutations contributing to any observed Dcas deletion-associated phenotypes, we used a number of discrete approaches to separately test the Dcas1 strain. First, we crossed Dcas1/Dcas1 stock to a stock containing the small Df(3L)Exel6083 deletion, which removes Dcas as well as Pk61c, CG6845, and CG7049 (Fig. 1A), to allow analysis of the phenotypes of Dcas1/Dcas1 versus Dcas1/Df(3L)Exel6083 flies. Second, we crossed the Dcas1/Dcas1 stock with a previously described DcasP1 hypomorphic allele [40] which has a GAL4-containing P-element inserted in the Dcas promoter, resulting in limited Dcas transcript levels, then analyzed Dcas1/DcasP1 flies. Third, in DcasP1/DcasP1 flies, we also introduced the DCas expressing a GAL4-activated UAS promoter fusion, a UAS-GFP-Dcas transgenic allele (as described in [40]), and assessed the DcasP1, UAS-GFP-Dcas/DcasP1, UAS-GFP-Dcas and DcasP1, UAS-GFP-Dcas/Dcas1 phenotypes. Fourth, we assessed the mRNA expression of Dcas and flanking genes in the Dcas1/Dcas1 and other mutant backgrounds.

While viable and fertile, the Dcas null stock yielded a a very weak lethal phenotype in which 10% of Dcas1/Dcas1 embryos did not hatch but instead developed a “kink” at stage 13, and arrested at stage 15–16 of embryonic development (Table 1, Fig. 1B). These embryos had germ band retraction (GBR) and dorsal closure (DC) defects [44], including an irregular leading edge of migrating cells (not shown); and typically had embryonal curvature and a posterior opening in the dorsal cuticle (Fig. 1C, Fig. 2). Similar GBR and DC phenotypes were seen in 6% of Dcas1/Df(3L)Exel6083 embryos and 1% of the Dcas1/DcasP1 embryos, as were similar rates of overall lethality. No lethality was observed in Dcas1/+ embryos (n = 613). Expression of GFP-Dcas in DcasP1, UAS-GFP-Dcas/DcasP1, UAS-GFP-Dcas and DcasP1, UAS-GFP-Dcas/Dcas1 embryos completely rescued embryonic GBR and DC defects observed in DcasP1/Dcas1 and Dcas1/Dcas1 stocks (not shown).

Figure 2
Genetic interactions of Dcas with Fak56D and Src42A.
Table 1
Synthetic lethal interactions involving Dcas1 and genes of the integrin signaling network.

Analysis of cDNA prepared from Dcas1/Dcas1 stocks indicated complete absence of Dcas transcript. DcasP1/DcasP1 mutants had significantly reduced but still detectable levels of the Dcas transcript (Figure 1D). While the Dcas1/Dcas1 stock had somewhat elevated expression of the adjacent CG7049 locus (which is predicted to encode a protein, but has no described phenotype or known function), the Dcas1/Df(3L)Exel6083 and DcasP1/DcasP1 stocks did not: indeed, gene expression of CG7049 was diminished in Df(3L)Exel6083/+ stock. Together, these expression results argue against variation in CG7049 expression as contributing to the observed GBR/DC phenotype (Figure 1D), and suggest the minimal phenotype observed with the DCasP1 allele reflect the fact that this strain reduces (to 43% of wt) but does not eliminate DCas mRNA expression.

Synthetic lethality of Dcas1 with FAK56 and Src42A mutations, and modifier interactions between Dcas and integrins

The best defined signaling partners of Cas proteins in mammals are components of the integrin signaling network. For instance, in mammals, interactions of the Cas proteins with FAK, Src, and integrins are critical for cell migration [1], [16]. We hypothesized that the weak Dcas1 phenotypes might be exacerbated by additional targeting of the Drosophila orthologs of these genes. The Drosophila FAK ortholog, Fak56D, is not essential for viability or fertility and a null mutation, Fak56CG1, has no gross phenotypes associated with cell migration [45], although homozygous mutations in Fak56D have been associated with morphogenesis of the optic stalk in second and third instar larvae [42]. Drosophila have two Src-related genes, Src42A and Src64, which have redundant function in GBR and DC (with double mutants having phenotypes similar to those seen in 10% of Dcas1/Dcas1 mutants, [46]), and other developmental processes [47]. Homozygous null alleles in Src42A have a high frequency of death before hatching or as first instar larvae, although some adult escapers of the hypomorphic allele Src42AJP45 have mild dorsal cleft phenotypes [46].

We first analyzed the genetic interactions of Dcas1 with Fak56CG1. We created a double-balanced stock which carried both Dcas1 and FAK56DCG1 mutations. Dcas1/Dcas1 in combination with either heterozygous or homozygous Fak56CG1 yielded no viable adult offspring (Table 1, Figure 2A). The Fak56CG1/Fak56CG1; Dcas1/+ genotype also significantly reduced the viability of adults. Analysis of the Fak56CG1/Fak56CG1; Dcas1/Dcas1 lethal phenotype indicated that most (95%) of the embryos did not hatch. The few escapers survived to pupal stages, but did not emerge. We then crossed double mutants to a stock with a green compound balancer CyO-TM3-GFP, which constitutively expresses GFP from the Hsp70 promoter during all developmental stages, and selected Fak56CG1, Dcas1/CyO-TM3-GFP embryos, to separate double homo- and heterozygotes for analysis of the cuticles of double homozygotes (Figs 2A). In contrast to embryos with either the Dcas1 or Fak56CG1 homozygotes, only 5% of Fak56CG1/Fak56CG1;Dcas1/Dcas1 mutants produced cuticles (Fig. 2B), and almost all observed cuticles were marked by dorsal and/or ventral holes, indicating dorsal closure defects. Additionally, Fak56CG1/Fak56CG1; Dcas1/Dcas1 cuticles had fused or missing (not shown) denticle belts, phenotypes never observed in cuticles of Fak56CG1 homozygotes alone.

Src42Ak10108 is a mild hypomorphic allele of Src42A: Src42Ak10108/Src42Ak10108 homozygous embryos hatch, but die as first instar larvae from defects in tail morphology, head involution, and tracheal necrosis [48]. However, we observed synthetic lethality in Dcas1/Dcas1; Src42Ak10108/CyO adult flies (Table 1, Figure 2A, C) and Dcas1/Dcas1; Src42Ak10108/Src42Ak10108 embryos, as fewer than 46% of these double mutant embryos hatched (data not shown). Cuticles were assessed by a strategy similar to that described for DCas1×Fak56DCG1 mutants. 90% of the cuticles of Src42Ak10108/Src42Ak10108; Dcas1/Dcas1 embryos had holes in or absence of the head cuticle, and 10% of Dcas1/Dcas1; Src42Ak10108/Src42Ak10108 cuticles had additional GBR defects. Similar phenotypes were obtained crossing Dcas1/Dcas1 to two additional Src42A mutant strains including the mild allele Src42Amiri and the strong allele Src42AE1 (Table 1 and not shown).

We confirmed the synthetic lethal interactions between DCas and Src42A and Fak56D, by in each case also assessing the phenotype of the Src and Fak alleles with Dcas1/Df(3L)Exel6083, in order to exclude the influence of potential secondary mutations in the Dcas1/Dcas1 stock. Fak56CG1/CyO; Dcas1/Df(3L)Exel6083 adults did not emerge, indicating complete lethality. Src42Ak10108/CyO; Dcas1/Df(3L)Exel6083 and Src42AE1/CyO; Dcas1/Df(3L)Exel6083 were semi-viable, emerging at approximately 50% of the rate of phenotypically normal adult siblings from the same cross (results not shown). Interestingly, the same cross to a double balanced DcasP1 allele did not result in the same substantial decrease in the numbers of Src42AE1/CyO; Dcas1/DcasP1 progeny, implying that moderate expression of Dcas is sufficient to support the survival of Src42AE1 mutants.

Interestingly, the low percentage of Src42Ak10108/+; Dcas1/Dcas1 and Src42AE1/+; Dcas1/Dcas1 adult escapers manifested wing blistering defects similar to those seen with mutants in integrin subunits [49] (Figure 3A). These data implied that simultaneous reduction in Dcas and Src42A function combined to impact an important integrin-dependent effector pathway. Based on these results, we also assessed whether Dcas interacted genetically with Drosophila orthologs of integrin α (mewEY09631 and mewG0429; IfB2 and If3) and β (mys1) subunits, which are upstream activators of SRC and FAK. Double balanced stocks of integrin mutants and Dcas1 were crossed to make double heterozygous stocks of each mutant in combination with Dcas, and analyzed for adult viability and visible phenotypes (Table 1).

Figure 3
Absence of Dcas induces wing defects in Src42A, If, and mew-deficient flies.

Loss of Dcas in If mutants only moderately affected viability of adult flies: 27% of If3/If3; Dcas1/Dcas1 and 56% of IfB2/+; Dcas1/Dcas1 emerge as adults (Figure 3B). However, the characteristic wing blistering defects of the If integrin α mutants [49] were significantly exacerbated in all viable progeny of double homozygous If3/If3; Dcas1/Dcas1 (Table 1, Figure 3B). Further, loss of a single or both copies of Dcas in combination with mewEY09631 (a viable weak hypomorphic allele) caused a dramatic reduction in the viability of adult mewEY09631 homozygotes (Table 1). Moreover, 2% of mewEY09631/+; Dcas1/Dcas1 flies had wing blisters and smaller, more rounded wings (Figure 3B). These interactions were enhanced using a lethal allele of mew (mewG0429), with viability of mewG0429/+; Dcas1/Dcas1 significantly reduced (Table 1). Finally, loss of Dcas significantly lowered the percentage of viable Dcas1/Dcas1; mys1/+ adults (Table 1), although no wing phenotypes were observed (not shown).

Dcas interacts with Fak56D to influence cell polarity and cytoskeleton

Based on the defined biology of mammalian Cas proteins (reviewed in [50]), the defects seen with Dcas and Fak56 mutant flies may reflect defects in cellular morphology (e.g., attachment and polarization) that inhibit appropriate migration during development. To begin to explore these mechanisms, we assessed the localization of markers of apical and basolateral polarity in flies with mutations in Dcas and Fak56. We compared localization of a set of polarity markers in embryos undergoing DC in mutants and wild type homozygotes and heterozygotes. Localization of polarity markers in heterozygous mutants was in all cases comparable to wild type (not shown). (Crumbs, CRB1) and aPKC localize to the subapical region/marginal zone in wild type embryos. For Crb, this localization was diminished in the 10% of phenotypically affected Dcas1/Dcas1 mutant embryos, while in Dcas1/Dcas1; Fak56CG1/Fak56CG1 Dcas1/Dcas1 embryos, Crb staining was generally reduced and diffuse in the cytoplasm (Fig 4A). aPKC staining was abnormally punctate specifically in the 10% of Dcas1/Dcas1embryos which had discernible GBR defects. Staining intensity of aPKC was both generally reduced and more cytoplasmically diffuse in Dcas1/Dcas1;Fak56CG1/Fak56CG1 embryos (Fig 4A).

Figure 4
Cell polarity consequences of mutations in Dcas and Fak56.

The septate junction markers Fas3 (fasciclin 3) and Dlg (Discs large), and an adherens junction marker, Shg (shotgun, E-cadherin), localize to the basolateral cell surface of epithelial cells. Fas3 expression and localization were unaffected in Dcas1/Dcas1; Fak56CG1/Fak56CG1 embryos beginning DC, although staining suggested a multi-layering of cells that was also indicated by the nuclear staining pattern obtained with the DNA label DRAQ5. Dlg staining patterns become more punctate and apical in Dcas1/Dcas1; Fak56CG1/Fak56CG1 embryos. Interestingly, Shg staining was markedly altered (Figs 4A–C) in embryos lacking Dcas, Fak56, or both. Shg staining in double mutant embryos was more cytoplasmic and diffuse compared to same stage embryos of other genotypes, with particular reduction of intense staining in the apical and lateral compartments. Detailed analysis of the intracellular distribution of Shg (Figs 4B, C) revealed significant reduction in the lateral punctate Shg staining in Dcas1/Dcas1; Fak56CG1/Fak56CG1 embryos. Although immunofluorescence analysis indicated Shg expression was maintained overall in Dcas null embryos, the 10% of embryos with GBR/DC defects had evidence of mislocalized Shg, with greater accumulation in a disorganized pool of Shg at the lateral and basal cell surface.

Dcas and Fak56 negatively regulate shg/E-cadherin protein localization in Drosophila embryos

The loss of Shg from the adherens junctional complex might reflect defects in localization of the protein, or reduced Shg expression. To discriminate these possibilities, we analyzed extracts made from Drosophila embryos (stage 13–16), 2nd–3rd instar larvae, and adults (Fig. 5A). Quantitive Western blot analysis indicated that Dcas1/Dcas1 embryos or larvae contain 2-fold higher levels of E-cadherin/Shg compared to WT, although no differences were seen in adult flies (Fig. 5A, graph). We next compared E-cadherin/Shg expression in Dcas1/Dcas1, Fak56CG1/Fak56CG1 or Dcas1/Dcas1;Fak56CG1/Fak56CG1 embryos. A Fak56CG1/Fak56CG1 genotype elevated E-cadherin protein levels to the same extent as Dcas1/Dcas1, while the double mutant had 3.1-fold more protein relative to wild type levels (Fig. 5B). E-cadherin transcription levels were not affected in Dcas and/or FAK mutants. The simplest interpretation of these results is that Shg does not effectively localize to lateral junctions in the absence of Dcas and Fak56. This defect initiates compensatory signals that modestly upregulate Shg at the level of translational control or protein stability, but this Shg remains trapped in the basal cytoplasmic cellular compartment.

Figure 5
Dcas negatively regulates expression of E-cadherin.

Interestingly, Crb has been reported to support Shg localization to adherens junctions [51]. The fact that the localization of Crb, Dlg, and Shg, but not Fas3, was strongly affected in the assessed double mutants indicated that Dcas and Fak56 did not ubiquitously affect localization controls. Further, in Drosophila, the Src orthologs genetically and functionally interact with shg, and phosphorylate the Shg partner protein armadillo (arm, β-catenin) promoting its degradation [47], [52]. As our data indicated Dcas both interacted with FAK56D and Src42A and resulted in mislocalized shg, these results together suggested close interactions between Dcas and Shg function.

Dcas genetically interacts with Shg

We therefore next assessed genetic interactions between the Dcas1 allele and loss-of-function alleles of shotgun (shg2, encoding an unstable protein that is prone to degradation [53]; shgE17B, a genetic null mutation producing a defective DE-cadherin; and shgK03401, produced by a P-element interruption of gene transcription) [54], and its functional partners armadillo (arm2, arm3, arm8,) and p120catenin (p120ctn308). Neither heterozygotic alleles of shg2, shgE17B p120ctn308 and arm2, nor double heterozygotes of Dcas1 and any of these genes produced visible phenotypes or reduced the emergence of adult flies (Figure 6 and Table 2). However, Dcas1/Dcas1 in combination with heterozygous shgK03401, arm3 or arm8, or homozygous p120ctn308, severely reduced viable adult progeny, as did combination of Dcas1/+ with p120ctn308/p120ctn308 (Figures 6A, 7A, 7B, and Table 2).

Figure 6
Genetic interactions of Dcas with shg.
Figure 7
Genetic interactions of Dcas with arm, shg and p120ctn.
Table 2
Synthetic lethal interactions involving Dcas1 and alleles of shg, arm, and p120ctn.

shg is important for morphogenesis of the head and ventral epithelium [53]. Although homozygous shg2 embryos complete DC due to abundant maternal contribution, some shg2/shg2 embryos may have small irregularities of the leading edge [53]. However, no shg2/shg2 embryos progress to 1st instar larvae because of moderate (49%, Fig. 6B, panels i versus ii) to severe (42% and 9%, Fig. 6B, panels iii and iv) defects in the embryonic head and ventral cuticle. By contrast, none of shg2/shg2; Dcas1/Dcas1 embryos hatched; rather, shg2/shg2; Dcas1/Dcas1 double homozygotes arrested in late embryogenesis. Although most of the embryos formed at least partial cuticles, absence of Dcas significantly enhanced shg2/shg2 cuticle defects, with all shg2/shg2; Dcas1/Dcas1 embryos showing severe defects that essentially eliminated head and ventral cuticle, while incomplete DC was reflected by the presence of holes in the dorsal cuticle (Fig. 6B, panel v).

To confirm specificity of the genetic interaction between Dcas and Shg, we subsequently crossed Dcas1 with two other alleles of Shg, shgE17B and shgK03401. Both alleles are embryonal lethal at embryonal stage 16, with embryos failing to produce head and ventral cuticle [53], [55]. Double mutants shgE17B/shgE17B; Dcas1/Dcas1 and shgK03401/shgK03401; Dcas1/Dcas1 were lethal or semi-lethal and had similarly enhanced cuticle defects, as observed with shg2/shg2; Dcas1/Dcas1, indicating the genetic interaction observed was not allele-specific.

Dcas interacts with arm and p120Ctn

Homozygous arm null alleles (arm2/arm2) have DC defects characterized by small holes in the dorsal epithelium (Fig. 7C) arm2/arm2 larvae also have a fully penetrant cuticle phenotype, characterized by shortened cuticle, severe segment polarity defects (resulting in lawn of denticles replacing well-separated denticle belts), a hole in the head region, and a naked cuticle from the anterior end to the third thoracic segment (Fig. 7C, panel iii) [56], [57]. 90% of arm2/arm2; Dcas1/Dcas1 flies had smaller cuticles than arm2/arm2 (Fig. 7C, panel iv). Among these, 82% completely lacked cuticle in the head region, and 65% had enhanced posterior curvature suggesting a strong GBR defect (Fig. 7C, panel v, vi). While 40% of arm2/arm2; Dcas1/Dcas1 flies retained the lawn of denticles characteristic of an arm2/arm2 mutant (compare Fig. 7C, panels iv and vi), 34% had complete deletion of ventral and dorsal denticle belts (Fig. 7C, panel vii), while 26% had well-separated posterior denticle belts (Fig. 7C, panel viii).

We extended our analysis to two additional alleles of arm (arm3 and arm8). Like arm2, these alleles express a truncated form of Armadillo [58], [59], due to either amino acid replacements resulting in a stop codon (arm2 and arm3) or p-element insertion (arm8) within the arm repeats. arm3 is embryonic lethal typically at stage 16, and is characterized by segment polarity and DC defects, while arm8 undergoes normal DC, but has strong segment polarity defects and dies in pupae. Dcas1 genetically interacts with both arm3 and arm8, as only 40% of the expected adult progeny with the genotypes arm3/FM7i-GFP, B; Dcas1/Dcas1 and arm8/FM7i-GFP, B; Dcas1/Dcas1 can be recovered (Table 2).

The p120-catenin homozygotes are viable and fertile; p120ctn308 mutation has been reported to induce a delayed, but complete DC and subtle irregularities of the leading edge in the majority of mutant embryos [60]. A p120ctn308/p120ctn308; Dcas1/Dcas1 genotype caused misalignment of segments and fused denticle belts (Fig. 7D, right panel, arrow), phenotypes not observed in p120ctn308/p120ctn308 mutants (Fig. 7D). Double mutant embryos p120ctn308/p120ctn308; Dcas1/Dcas1 successfully complete embryogenesis and form larvae, but produce few pupae and no adult flies (Figure 7B and Table 2). The later point of lethality may indicate a less direct interaction than that between Dcas, shg, and arm.

Specificity of Dcas genetic interactions

To rule out the possibility of secondary hits accumulated during double balancing and multiple crosses influencing phenotypes, we chose strongest shg and arm alleles (shg2, shgE17B and arm2) double balanced with Dcas1 (shg2/CyO;Dcas1/TM6B,Ubx,y+,shgE17B/CyO; Dcas1/TM6B,Ubx,y+,arm2/FM7i-GFP,B; Dcas1/TM6B,AntHu,y+) and crossed to Df(3L)Exel6083/TM6B,Ubx,y+. No progeny with Dcas1/Df(3L)Exel6083 emerged from these crosses, indicating that Dcas is indeed indispensible for survival of shg and arm mutants. When same double balanced flies were crossed to DcasP1, less than 50% of shgE17B/CyO;Dcas1/DcasP1 or shgE17B/CyO;Dcas1/DcasP1 adults expected from the cross emerged (data not shown), indicating sensitivity of shg mutants to even slight loss of Dcas expression.

Finally, we also explored other potential Dcas genetic interactions suggested from studies of the mammalian Cas paralogs NEDD9 and BCAR1. In mammals, NEDD9 interacts with Aurora-A kinase to regulate cell cycle [61], while BCAR1 interacts with the adaptor protein NCK in growth factor signaling [62]. Combination of Dcas1 with mutants in the Drosophila ortholog of Aurora-A (the amorphic alleles Aur1 or Aur87Ac-3) or of Nck (dreadlocks, the amorphic dock04723 allele) resulted in no synthetic lethality (Table S1). These negative results suggest a more ancestral and specific relationship of Dcas with the other genes yielding positive phenotypes.


This work identifies a strong interaction between the Dcas, and integrin pathway genes, including integrins and their effector kinases Fak56D and Src42A, during early embryonal development in Drosophila. The synthetic lethal phenotypes found in double mutants of Dcas and Src or FAK56D were marked by defects in dorsal closure and in some cases by the appearance of anterior cuticle holes that suggested head involution defects. These defects were commonly accompanied by abnormalities in epithelial function, including failure to appropriately localize shg/E-cadherin to cell junctions, and reduced shg expression. Our data are compatible with the idea that either Fak56D or Dcas is sufficient to support shg/E-cadherin localization and cell polarization during morphogenetic movements in Drosophila embryos, but the absence of both cannot be sustained.

Building from these observations, we established a novel synthetic lethal relationship between DCas, shg, and arm. As with crosses to alleles of Fak56D and Src42A, the point of lethality was at the time of dorsal closure, at embryonal stages 15–16, and associated with defective cuticle formation. One way to integrate these observations is to hypothesize that the DCas, Fak56D, and Shg protein products are normally in dynamic balance, with Dcas regulating Shg cycling. The fact that Crb and Dlg1, a mammalian homolog of Dlg, have been reported to support Shg localization to adherens junctions [51], [63], suggests that Dcas/Fak56/Src42A specifically interact to support this cell polarity/cell junctional control system. In this context, it is suggestive that the Crb family protein CRB3 has been described as part of a complex including CRB3, Pals1, and PatJ that becomes tightly associated with Src kinase during reorganization of cell polarity [64]. In the absence of DCas and Fak56D, Shg cannot localize properly; the moderately elevated levels of Shg proteins found in these embryos most likely arises as part of a cellular compensatory mechanism in response to decreased functional Shg signaling complexes. In further indirect support of the idea that this is a specific Dcas action, the fact that genetic interactions were not observed between Dcas1 and Aur or Dock indicates that Dcas does not promiscuously interact with other genetic lesions to reduce viability.

A previous study demonstrated a role for Dcas in axonal guidance in the development of the nervous system of adult flies [40]. That work analyzed the hypomorphic Dcas mutant allele DcasP1, and the small deficiency Df(3L)Exel6083, including Dcas and five adjacent genes, which we have also used in this study. The earlier study focused exclusively on analyzing the contribution of Dcas to axonal guidance in late (stage 16/17) embryos: in that analysis, Dcas functioned similarly to integrins, and genetically interacted with integrins (if, mew, and mys) in regulating axon guidance and axonemal defasciculation. In this context, it is intriguing that the mammalian Cas family NEDD9 gene is abundant during neuronal development, has been proposed as a candidate locus for oral cleft defects in humans based on its chromosomal location near the OFC-1 locus [65], and has recently been implicated in control of neural migration and neuronal cell fate [66], [67]. Together these findings raise the possibility that this specific Dcas paralog has a specific role in human neuronal migration and morphogenesis of the head. As with our data using the new Dcas1 allele, homozygous deletion of Dcas in conjunction with integrins had moderate effect on viability of adult flies, although our work for the first time demonstrates an interaction between Dcas and if and mew, and also between Dcas and Src, in regulation of wing development.

Generation of the first null allele of Dcas provides a useful new tool to study the role of this protein in Drosophila development. This work illuminates the evolutionary conservation of Dcas function within the integrin and receptor tyrosine kinase network, including FAK, Src, and integrins genes. The finding that a low percentage of embryos with mutant Dcas and all embryos with double mutations in Dcas and Fak56D, have perturbed localization of polarity markers, including Shg, indicates a novel function for Cas family in regulation of cell polarity. To date, the evidence directly connecting Cas proteins to a known mechanism for control of cell polarity is sparse. Although NEDD9 was in fact discovered in a functional genomics screen for cell cycle and polarity modifiers in budding yeast (leading to its designation as HEF1, Human Enhancer of Filamentation 1) [5], the mechanism involved was not established, and given the great evolutionary distance involved, may not be relevant to a role in metazoans. Both BCAR1 and NEDD9 interact physically with proteins that influence cell polarity controls during pseudopod extension and other actin polarization processes: these include the GTP exchange factor AND-34 [68] and Rac1 [69].

Our data in the present study indicating genetic interactions with cell-cell junction regulatory proteins Shg, Arm and p120-catenin may have considerable significance in the sphere of cancer research, as it implies that overexpression of Cas proteins may promote cancer progression by influencing the polarized movement of cells and influencing lateral attachments. The fact that one report has indicated interactions between BCAR1 and nephrocystins at cell-cell junctions in polarized epithelial cells [70] implies that a potentially direct interaction of Cas proteins in these structures is conserved through mammals. However, given the known interactions of Cas proteins with FAK and SRC at focal adhesions, another possibility is that Cas may additionally or alternatively impact Shg function through indirect signaling emanating from these structures. Notably, Bui et al. recently reported that NEDD9 overexpression induced by dioxin caused downregulation of E-cadherin [37], and it will be of great interest to study the consequences of overexpressing Dcas on Drosophila development. Consequences for loss of NEDD9 expression on E-cadherin expression or localization are not yet known. Resolving these questions will provide intriguing directions for future studies.

Materials and Methods

D. melanogaster stocks, crosses

The following mutant Drosophila stocks were obtained at Bloomington Stock Center and are described in Flybase ( shg2, shgK03401, shgE17B arm2, arm3, arm8, Src42A10108k, Src42AJP45, Src42AE1, src42Amiri, aur1, aur87Ac-3, dock04723 and p120ctn308, mewEY09631, IfB2, If3, mewG0429, mys1. The fak56DCG1 strain was obtained from Ruth H. Palmer (Umea University, Sweden). The stock containing the DcasP1 allele was provided by Dr. Kolodkin (Johns Hopkins School of Medicine, Baltimore). Green double balancer Fm7i, B, Kr::GFP/+; ki/TM6B, Tb, Kr::GFP was used for double balancing Dcas and genes located on X chromosome. Balancer stocks Tm3, Sb'/Tm6, Dr', w, TM2, Ubx'/Tm6, Sb' and yw, Sco/CyO; ki/TM6B, Ubx, y+ and green compound double-balancer w1; T(2;3)CyO-TM3, P{GAL4-Hsp70.PB}TR1, P{UAS-GFP.Y}TR1; P{GAL4-Hsp70.PB}TR2, P{UAS-GFP.Y} TR2, y+ Ser1/nocSco; Sb1 stocks from Bloomington Stock Center were used to balance the null Dcas1 mutation. To create double balanced If, mys and mew and Dcas stocks, we used the double balancer FM7i, B, Kr::GFP; ki/TM6B, Tb, Kr::GFP, which constitutively expresses GFP on chromosomes X and III. FAK56D, Src42A and other chromosome II mutants were double balanced with yw; Elp/CyO; ki/TM6B, Ubx, y+ green balancer. Double balanced mutant alleles were then crossed to double-balanced Dcas alleles, i.e Dcas1. We also attempted to generate double mutants in Dcas and Src64B. Unfortunately, the very close location of the Dcas and Src64B loci prevented successful recombination involving these mutations.

Construction of CG1212/Dcas knockout and viability calculations

To generate a Dcas null allele, yw hs-flp; FRT82neurIF63/Tm3, Sb' females were crossed to FRT-containing PBac{WH}f00059 (BDSC, Bloomington, IN) males to produce yw hs-flp/Y; PBac{WH}f00059/Tm3, Sb' males, which were backcrossed to yw hs-flp; FRT82neurIF63/Tm3, Sb'. Next, yw hs-flp; PBac{WH}f00059/Tm3, Sb' females were crossed with w, P5-HA-2428 males (Szeged Drosophila Stock Centre, Hungary). Male progeny with the genotype yw hs-flp/Y; PBac{WH}f00059/P5-HA-2428 were backcrossed to yw hs-flp; PBac{WH}f00059/Tm3, Sb' to obtain yw hs-flp; PBac{WH}f00059/P{RS5}5-HA-2428 flies. We then initiated double stranded breaks and isolated knockouts as described in [71]. Endpoints of excision were defined by the P-element P{RS5}5-HA-2428, positioned within 50bp from the Dcas start codon and containing an FRT site in the same orientation as the piggyBac Pbac{WH}f00059 transposon, located in between the Dcas ORF and the adjacent downstream gene CG7049 (Fig. 1A). Flippase-activated excision produced 20 potential mutant stocks, which were then analyzed by quantitative RT-PCR with seven sets of primers spanning the Dcas coding region, and in flanking genes (Fig. 1A). Correct endpoints of the Dcas deletion were initially confirmed using qRT-PCR to analyze DNA from adult flies, using primers directed at the promoter, and first and last coding exons of Dcas, as well as flanking upstream and downstream chromosomal sequences, to confirm that the Dcas gene was not detectable in Dcas1/Dcas1 mutant stocks, although readily detected in WT flies. Dcas transcript levels were also measured in knockout flies using qRT-PCR to analyze at least 3 independent samples of RNA prepared using the RNeasy kit (Qiagen) from adult flies and larvae. Dcas1 null flies were serially backcrossed to 3rd chromosome balancer stocks (TM3,TM6 and TM2) to exclude additional recombination-associated mutations on other chromosomes before further characterization.

Double balanced heterozygous adults containing mutations in Dcas and prospective interacting genes were selected and crossed together to establish stocks and to assess viability of adult progeny. The total number of expected progeny was calculated from the number of phenotypically viable double balanced adult heterozygotes, i.e. Fak56CG1/CyO; Dcas1/TM6B, Ubx, y+, which were considered 100% viable. The percentage of viability for the rest of the progeny was calculated in agreement with Mendel's law of independent assortment for two alleles, which was also used to calculate the ratio between different genotypes in the progeny. If both mutant alleles were viable, i.e. Fak56CG1 and Dcas1, the ratios were as follows: Fak56CG1/CyO; Dcas1/TM6B, Ubx, y+: Fak56CG1/Fak56CG1; Dcas1/TM6B, Ubx, y+: Fak56CG1/CyO; Dcas1/Dcas1: Fak56CG1/Fak56CG1; Dcas1/Dcas1 as 4[ratio]2[ratio]2[ratio]1. If one of mutants alleles was lethal, i.e. in a combination of SrcK10108 and Dcas1, the SrcK10108/CyO; Dcas1/TM6B, Ubx, y+: SrcK10108/CyO; Dcas1/Dcas1 ratio was 2[ratio]1. Progeny from more than three independent crosses was collected and represented as tables modeled after [46].

Preparation of embryos and immunohistochemistry

For analysis of localization of polarity markers, embryos were prepared as described by [72], with minor modifications. Briefly, embryos collected off apple-agar plates were washed in 50% bleach for 2 minutes, then rinsed twice in PBS and gently shaken on a platform for 40 minutes in 1[ratio]1 8% PFA/heptane mixture containing 2 units/ml of phalloidin (Invitrogen, Carlsbad, CA). Embryos accumulating at the interface between PFA and heptane were collected, applied to double stick tape, then de-vitellinated with a fine glass needle. Rehydrated embryos were blocked with 10% BSA/PBS for an hour, washed in 1% BSA/PBS, and incubated with a primary antibody for 2 hours, followed by two 5-minute washes in PBS, and incubation with secondary antibody for an hour. Embryos were visualized with Leica TCS SL and Nikon C1 confocal microscopes, and images analyzed using Metamorph and EZ-C1 freeViewer software.

Western blot analysis

Whole embryo, larval and fly lysates were prepared by homogenization in 3× Laemmli sample buffer containing 10% SDS, and then boiling for 5 minutes. Samples were separated by 10% Bis-Tris NuPage PAGE (Invitrogen, Carlsbad, CA). Western blots were performed using standard protocols.

Antibodies and visualization reagents

Primary antibodies used included ECCD-2 mouse α-E-cadherin (Invitrogen, Carlsbad, CA), rat E-cadherin, mouse α-Fasciclin3, rabbit α-crumbs (DSHB, Iowa), α-zeta-PKC and α-Dlg (Santa Cruz Biotechnology, Inc, Santa Cruz, CA), mouse HRP-conjugated β-actin (Abcam, Cambridge, MA). Secondary antibodies included HRP-conjugated α-mouse, -rat or –rabbit (Amersham, Pittsburgh, PA) or Alexa-fluor-488, -568 or -633-conjugated α-mouse, -rat or –rabbit ((Invitrogen, Carlsbad, CA). Nuclei were stained with DRAQ5 reagent (Cell Signaling, Boston, MA).

Cuticle preparation

Embryos were collected for 26 hours after the parents were removed from the apple-agar plates, dechorionated with 50% bleach, devitellinized in 1[ratio]1 heptane/methanol for 15 minutes, washed 2× with methanol, 2× with lactic acid, transferred on a slide into a drop of Hoyer's medium, and photographed using a phase contrast microscope (Nikon Eclipse TE-2000-U). The stocks carrying mutations in a gene of interest and Dcas were rebalanced over a green compound balancer to separate GFP-negative double homozygotes and GFP-positive double heterozygotes. Homozygotes were then collected for cuticle preparations. Where applicable, GFP-negative homozygotes and GFP-positive heterozygotes were separated using fluorescent dissecting microscope, prior to bleaching.

Wing preparation

Wings were detached and mounted into Hoyer's medium. Images were taken at 4× magnification on Leica TCS SL microscope.

Embryo Hatch Rate Analysis

Mutant embryos were collected from indicated crosses. For hatch rate determination, embryos were collected on apple-agar plates for 4 hr, than the parents were removed and more than 500 embryos per genotype were counted after 2 days' incubation.

Real Time PCR analysis

Stage 13–15 embryos were bleached and rinsed with distilled water. 30 mg of embryos were used to isolate mRNA with the RNAeasy kit (Qiagen, Valencia, CA) and overall mRNA quality assessed using an Agilent Bioanalyzer (Agilent, Santa Clara, CA). The concentration of Shg mRNA in was quantified via real-time PCR with the Smartcycler detection system (Cepheid, Sunnyvale, CA) using SYBR green I (Molecular Probe, Eugene, OR) in three independent experiments. The primers used in the PCR reaction were as follows: Shotgun, forward primer 5′- GCGCTACGACGAATCCATG-3′ and reverse primer 5′- AGATAATACCCGACTCCTTGTCAATC-3′; and as a normalization control, the housekeeping gene RpII140, forward primer 5′-CGCACGTGGAAGTTGGTAAT-3′ and reverse primer 5′- ACAATCAGAGTCCGCGTA ACAC-3′.

Supporting Information

Table S1

Additional genetic interactions of Dcas1. For data shown, the parental crosses for Dcas1 and dock04723 were performed as described in Materials and Methods. Alleles of Aurora kinase (aur1 and aur87Ac-3) were first recombined to position both mutations to the same chromosome with Dcas1, balanced over TM3, Ser balancer to establish a double heterozygous stock (i.e. aur1, Dcas1/TM3). Double heterozygotes were crossed with Dcas1/Dcas1 to produce aur1, Dcas1/Dcas1, aur87Ac-3, and Dcas1/Dcas1 which were then crossed back to double heterozygotes. The viable progeny of indicated genotypes was collected and compared to phenotypically normal double heterozygous siblings, (i.e. aur1, Dcas1/TM3) in each of 3 independent experiments.

(0.03 MB DOC)


We are grateful to Ruth H. Palmer for the FAK56D stock, and to Alex Kolodkin for the DcasP1 stock. We thank Emmanuelle Nicolas of the Fox Chase Cancer Center Genomics Facility for quantitative PCR analysis. We thank Wendy Yun, Diana Zitserman, Tony Tong and Elena Kotova for technical assistance and advice. We thank Dr. Alana O'Reilly for extremely helpful comments on the manuscript. The monoclonal antibodies to rat E-cadherin, mouse α-Fasciclin3 and rabbit α-Crumbs (developed by T. Uemura, C. Goodman and E. Knust, respectively) were obtained from the Developmental Studies Hybridoma Bank developed under the auspices of the NICHD and maintained by The University of Iowa, Department of Biology, Iowa City, IA 52242.


Competing Interests: The authors have declared that no competing interests exist.

Funding: This work was supported by National Institutes of Health (NIH) R01s CA63366 and CA113342, and by Pennsylvania Tobacco Settlement Funds (to EAG), and by an appropriation from the Commonwealth of Pennsylvania, by NIH core grant CA06927 (to Fox Chase Cancer Center) and support from the Pew Charitable Fund (to Fox Chase Cancer Center). Alexei Tulin was supported by R01 GM077452, and FR by R01 NS059971. The funders had no role in study design, data collection and analysis, decision to publish, or preparation of the manuscript.


1. Defilippi P, Di Stefano P, Cabodi S. p130Cas: a versatile scaffold in signaling networks. Trends Cell Biol. 2006;16:257–263. [PubMed]
2. Singh M, Cowell L, Seo S, O'Neill G, Golemis E. Molecular basis for HEF1/NEDD9/Cas-L action as a multifunctional co-ordinator of invasion, apoptosis and cell cycle. Cell Biochem Biophys. 2007;48:54–72. [PMC free article] [PubMed]
3. Tikhmyanova N, Little JL, Golemis EA. CAS proteins in normal and pathological cell growth control. Cell Mol Life Sci 2009 [PMC free article] [PubMed]
4. Sakai R, Iwamatsu A, Hirano N, Ogawa S, Tanaka T, et al. A novel signaling molecule, p130, forms stable complexes in vivo with v-Crk and v-Src in a tyrosine phosphorylation-dependent manner. EMBO J. 1994;13:3748–3756. [PubMed]
5. Law SF, Estojak J, Wang B, Mysliwiec T, Kruh GD, et al. Human Enhancer of Filamentation 1 (HEF1), a novel p130Cas-like docking protein, associates with FAK, and induces pseudohyphal growth in yeast. Mol Cell Biol. 1996;16:3327–3337. [PMC free article] [PubMed]
6. Ishino M, Ohba T, Sasaki H, Sasaki T. Molecular cloning of a cDNA encoding a phosphoprotein, Efs, which contains a Src homology 3 domain and associates with Fyn. Oncogene. 1995;11:2331–2338. [PubMed]
7. Singh MK, Dadke D, Nicolas E, Serebriiskii IG, Apostolou S, et al. A Novel Cas Family Member, HEPL, Regulates FAK and Cell Spreading. Mol Biol Cell. 2008;19:1627–1636. [PMC free article] [PubMed]
8. O'Neill GM, Fashena SJ, Golemis EA. Integrin signaling: a new Cas(t) of characters enters the stage. Trends Cell Biol. 2000;10:111–119. [PubMed]
9. Klemke RL, Leng J, Molander R, Brooks PC, Vuori K, et al. CAS/Crk coupling serves as a “molecular switch” for induction of cell migration. J Cell Biol. 1998;140:961–972. [PMC free article] [PubMed]
10. Simpson KJ, Selfors LM, Bui J, Reynolds A, Leake D, et al. Identification of genes that regulate epithelial cell migration using an siRNA screening approach. Nat Cell Biol. 2008;10:1027–1038. [PubMed]
11. Natarajan M, Hecker TP, Gladson CL. FAK signaling in anaplastic astrocytoma and glioblastoma tumors. Cancer J. 2003;9:126–133. [PubMed]
12. Kim M, Gans JD, Nogueira C, Wang A, Paik JH, et al. Comparative oncogenomics identifies NEDD9 as a melanoma metastasis gene. Cell. 2006;125:1269–1281. [PubMed]
13. van Seventer GA, Salman HJ, Law SF, O'Neill GM, Mullen MM, et al. Focal adhesion kinase regulates beta1 integrin dependent migration through an HEF1 effector pathway. Eur J Imm. 2001;31:1417–1427. [PubMed]
14. Honda H, Nakamoto T, Sakai R, Hirai H. p130(Cas), an assembling molecule of actin filaments, promotes cell movement, cell migration, and cell spreading in fibroblasts. Biochem Biophys Res Commun. 1999;262:25–30. [PubMed]
15. Cary LA, Han DC, Polte TR, Hanks SK, Guan J-L. Identification of p130Cas as a mediator of focal adhesion kinase-promoted cell migration. J Cell Biol. 1998;140:211–221. [PMC free article] [PubMed]
16. O'Neill GM, Seo S, Serebriiskii IG, Lessin SR, Golemis EA. A new central scaffold for metastasis: parsing HEF1/Cas-L/NEDD9. Cancer Res. 2007;67:8975–8979. [PMC free article] [PubMed]
17. Honda H, Oda H, Nakamoto T, Honda Z, Sakai R, et al. Cardiovascular anomaly, impaired actin bundling and resistance to Src-induced transformation in mice lacking p130Cas. Nat Genet. 1998;19:361–365. [PubMed]
18. Fashena SJ, Einarson MB, O'Neill GM, Patriotis CP, Golemis EA. Dissection of HEF1-dependent functions in motility and transcriptional regulation. J Cell Sci. 2002;115:99–111. [PubMed]
19. Brabek J, Constancio SS, Siesser PF, Shin NY, Pozzi A, et al. Crk-associated substrate tyrosine phosphorylation sites are critical for invasion and metastasis of SRC-transformed cells. Mol Cancer Res. 2005;3:307–315. [PubMed]
20. Cabodi S, Tinnirello A, Di Stefano P, Bisaro B, Ambrosino E, et al. p130Cas as a new regulator of mammary epithelial cell proliferation, survival, and HER2-neu oncogene-dependent breast tumorigenesis. Cancer Res. 2006;66:4672–4680. [PubMed]
21. Sanz-Moreno V, Gadea G, Ahn J, Paterson H, Marra P, et al. Rac activation and inactivation control plasticity of tumor cell movement. Cell. 2008;135:510–523. [PubMed]
22. Liu X, Elia AEH, Law SF, Golemis EA, Farley J, et al. A novel ability of Smad3 to regulate proteasomal degradation of a Cas family member, HEF1. EMBO J. 2000;19:6759–6769. [PubMed]
23. Zheng M, McKeown-Longo PJ. Regulation of HEF1 expression and phosphorylation by TGF-beta 1 and cell adhesion. J Biol Chem. 2002;277:39599–39608. [PubMed]
24. Inamoto S, Iwata S, Inamoto T, Nomura S, Sasaki T, et al. Crk-associated substrate lymphocyte type regulates transforming growth factor-beta signaling by inhibiting Smad6 and Smad7. Oncogene 2006 [PubMed]
25. Feng L, Guedes S, Wang T. AIP4/hItch is an Ubiquitin E3 ligase For HEF1 In TGF-{beta} signaling pathways. J Biol Chem 2004
26. Nourry C, Maksumova L, Pang M, Liu X, Wang T. Direct Interaction Between Smad3, APC10, CDH1 and HEF1 in Proteasomal Degradation of HEF1. BMC Cell Biol. 2004;5:20. [PMC free article] [PubMed]
27. Brinkman A, van der Flier S, Kok EM, Dorssers LC. BCAR1, a human homologue of the adapter protein p130Cas, and antiestrogen resistance in breast cancer cells. J Natl Cancer Inst. 2000;92:112–120. [PubMed]
28. van der Flier S, Brinkman A, Look MP, Kok EM, Meijer-Van Gelder ME, et al. Bcar1/p130Cas protein and primary breast cancer: prognosis and response to tamoxifen treatment. J Natl Cancer Inst. 2000;92:120–127. [PubMed]
29. Minegishi M, Tachibana K, Sato T, Iwata S, Nojima Y, et al. Structure and function of Cas-L, a 105-kD Crk-associated substrate-related protein that is involved in beta-1 integrin-mediated signaling in lymphocytes. J Exp Med. 1996;184:1365–1375. [PMC free article] [PubMed]
30. Astier A, Manie SN, Law SF, Canty T, Hagheyeghi N, et al. Association of the Cas-like molecule HEF1 with CrkL following integrin and antigen receptor signaling in B cells. Possible relevance to neoplastic lymphohematopoietic cells. Leuk Lymph. 1997;28:65–72. [PubMed]
31. Manie SN, Beck ARP, Astier A, Law SF, Canty T, et al. Involvement of p130Cas and p105HEF1, a novel Cas-like docking protein, in a cytoskeleton-dependent signaling pathway initiated by ligation of integrin or antigen receptor on human B cells. J Biol Chem. 1997;272:4230–4236. [PubMed]
32. Sattler M, Salgia R, Shrikhande G, Verma S, Uemura N, et al. Differential signaling after beta1 integrin ligation is mediated through binding of CRKL to p120CBL and p110HEF1. J Biol Chem. 1997;272:14320–14326. [PubMed]
33. Kim SH, Xia D, Kim SW, Holla V, Menter DG, et al. Human enhancer of filamentation 1 Is a mediator of hypoxia-inducible factor-1alpha-mediated migration in colorectal carcinoma cells. Cancer Res. 2010;70:4054–4063. [PMC free article] [PubMed]
34. Lucas JT, Jr, Salimath BP, Slomiany MG, Rosenzweig SA. Regulation of invasive behavior by vascular endothelial growth factor is HEF1-dependent. Oncogene 2010 [PMC free article] [PubMed]
35. Natarajan M, Stewart JE, Golemis EA, Pugacheva EN, Alexandropoulos K, et al. HEF1 is a necessary and specific downstream effector of FAK that promotes the migration of glioblastoma cells. Oncogene. 2006;25:1721–1732. [PubMed]
36. Ji H, Ramsey MR, Hayes DN, Fan C, McNamara K, et al. LKB1 modulates lung cancer differentiation and metastasis. Nature. 2007;448:807–810. [PubMed]
37. Bui LC, Tomkiewicz C, Chevallier A, Pierre S, Bats AS, et al. Nedd9/Hef1/Cas-L mediates the effects of environmental pollutants on cell migration and plasticity. Oncogene. 2009;28:3642–3651. [PubMed]
38. Izumchenko E, Singh MK, Plotnikova OV, Tikhmyanova N, Little JL, et al. NEDD9 promotes oncogenic signaling in mammary tumor development. Cancer Res. 2009;69:7198–7206. [PMC free article] [PubMed]
39. Seo S, Asai T, Saito T, Suzuki T, Morishita Y, et al. Crk-associated substrate lymphocyte type is required for lymphocyte trafficking and marginal zone B cell maintenance. J Immunol. 2005;175:3492–3501. [PubMed]
40. Huang Z, Yazdani U, Thompson-Peer KL, Kolodkin AL, Terman JR. Crk-associated substrate (Cas) signaling protein functions with integrins to specify axon guidance during development. Development. 2007;134:2337–2347. [PubMed]
41. Tomancak P, Berman BP, Beaton A, Weiszmann R, Kwan E, et al. Global analysis of patterns of gene expression during Drosophila embryogenesis. Genome Biol. 2007;8:R145. [PMC free article] [PubMed]
42. Murakami S, Umetsu D, Maeyama Y, Sato M, Yoshida S, et al. Focal adhesion kinase controls morphogenesis of the Drosophila optic stalk. Development. 2007;134:1539–1548. [PubMed]
43. Xie HB, Golic KG. Gene deletions by ends-in targeting in Drosophila melanogaster. Genetics. 2004;168:1477–1489. [PubMed]
44. Schock F, Perrimon N. Cellular processes associated with germ band retraction in Drosophila. Dev Biol. 2002;248:29–39. [PubMed]
45. Grabbe C, Zervas CG, Hunter T, Brown NH, Palmer RH. Focal adhesion kinase is not required for integrin function or viability in Drosophila. Development. 2004;131:5795–5805. [PubMed]
46. Tateno M, Nishida Y, Adachi-Yamada T. Regulation of JNK by Src during Drosophila development. Science. 2000;287:324–327. [PubMed]
47. Takahashi M, Takahashi F, Ui-Tei K, Kojima T, Saigo K. Requirements of genetic interactions between Src42A, armadillo and shotgun, a gene encoding E-cadherin, for normal development in Drosophila. Development. 2005;132:2547–2559. [PubMed]
48. Lu X, Li Y. Drosophila Src42A is a negative regulator of RTK signaling. Dev Biol. 1999;208:233–243. [PubMed]
49. Bloor JW, Brown NH. Genetic analysis of the Drosophila alphaPS2 integrin subunit reveals discrete adhesive, morphogenetic and sarcomeric functions. Genetics. 1998;148:1127–1142. [PubMed]
50. Tikhmyanova N, Little JL, Golemis EA. CAS proteins in normal and pathological cell growth control. Cell Mol Life Sci. 2010;67:1025–1048. [PMC free article] [PubMed]
51. Klebes A, Knust E. A conserved motif in Crumbs is required for E-cadherin localisation and zonula adherens formation in Drosophila. Curr Biol. 2000;10:76–85. [PubMed]
52. Shindo M, Wada H, Kaido M, Tateno M, Aigaki T, et al. Dual function of Src in the maintenance of adherens junctions during tracheal epithelial morphogenesis. Development. 2008;135:1355–1364. [PubMed]
53. Uemura T, Oda H, Kraut R, Hayashi S, Kotaoka Y, et al. Zygotic Drosophila E-cadherin expression is required for processes of dynamic epithelial cell rearrangement in the Drosophila embryo. Genes Dev. 1996;10:659–671. [PubMed]
54. Tepass U, Gruszynski-DeFeo E, Haag TA, Omatyar L, Torok T, et al. shotgun encodes Drosophila E-cadherin and is preferentially required during cell rearrangement in the neurectoderm and other morphogenetically active epithelia. Genes Dev. 1996;10:672–685. [PubMed]
55. Dumstrei K, Wang F, Shy D, Tepass U, Hartenstein V. Interaction between EGFR signaling and DE-cadherin during nervous system morphogenesis. Development. 2002;129:3983–3994. [PubMed]
56. Wieschaus E, Riggleman R. Autonomous requirements for the segment polarity gene armadillo during Drosophila embryogenesis. Cell. 1987;49:177–184. [PubMed]
57. Peifer M, Wieschaus E. The segment polarity gene armadillo encodes a functionally modular protein that is the Drosophila homolog of human plakoglobin. Cell. 1990;63:1167–1176. [PubMed]
58. Cox RT, Pai LM, Miller JR, Orsulic S, Stein J, et al. Membrane-tethered Drosophila Armadillo cannot transduce Wingless signal on its own. Development. 1999;126:1327–1335. [PubMed]
59. Cox RT, Kirkpatrick C, Peifer M. Armadillo is required for adherens junction assembly, cell polarity, and morphogenesis during Drosophila embryogenesis. J Cell Biol. 1996;134:133–148. [PMC free article] [PubMed]
60. Myster SH, Cavallo R, Anderson CT, Fox DT, Peifer M. Drosophila p120catenin plays a supporting role in cell adhesion but is not an essential adherens junction component. J Cell Biol. 2003;160:433–449. [PMC free article] [PubMed]
61. Pugacheva EN, Golemis EA. The focal adhesion scaffolding protein HEF1 regulates activation of the Aurora-A and Nek2 kinases at the centrosome. Nat Cell Biol. 2005;7:937–946. [PMC free article] [PubMed]
62. Rivera GM, Antoku S, Gelkop S, Shin NY, Hanks SK, et al. Requirement of Nck adaptors for actin dynamics and cell migration stimulated by platelet-derived growth factor B. Proc Natl Acad Sci U S A. 2006;103:9536–9541. [PubMed]
63. Reuver SM, Garner CC. E-cadherin mediated cell adhesion recruits SAP97 into the cortical cytoskeleton. J Cell Sci. 1998;111 ( Pt 8):1071–1080. [PubMed]
64. Wong EW, Mruk DD, Lee WM, Cheng CY. Par3/Par6 polarity complex coordinates apical ectoplasmic specialization and blood-testis barrier restructuring during spermatogenesis. Proc Natl Acad Sci U S A. 2008;105:9657–9662. [PubMed]
65. Beaty TH, Fallin MD, Hetmanski JB, McIntosh I, Chong SS, et al. Haplotype diversity in 11 candidate genes across four populations. Genetics. 2005;171:259–267. [PubMed]
66. Aquino JB, Lallemend F, Marmigere F, Adameyko, Golemis EA, et al. The retinoic acid inducible Cas-family signaling protein Nedd9 regulates neural crest cell migration by modulating adhesion and actin dynamics. Neuroscience 2009 [PMC free article] [PubMed]
67. Vogel T, Ahrens S, Buttner N, Krieglstein K. Transforming Growth Factor {beta} Promotes Neuronal Cell Fate of Mouse Cortical and Hippocampal Progenitors In Vitro and In Vivo: Identification of Nedd9 as an Essential Signaling Component. Cereb Cortex 2009 [PMC free article] [PubMed]
68. Cai D, Felekkis KN, Near RI, O'Neill GM, van Seventer JM, et al. The GDP exchange factor AND-34 is expressed in B cells, associates with HEF1, and activates Cdc42. J Immunol. 2003;170:969–978. [PubMed]
69. Cho SY, Klemke RL. Purification of pseudopodia from polarized cells reveals redistribution and activation of Rac through assembly of a CAS/Crk scaffold. J Cell Biol. 2002 in press. [PMC free article] [PubMed]
70. Donaldson JC, Dempsey PJ, Reddy S, Bouton AH, Coffey RJ, et al. Crk-associated substrate p130(Cas) interacts with nephrocystin and both proteins localize to cell-cell contacts of polarized epithelial cells. Exp Cell Res. 2000;256:168–178. [PubMed]
71. Parks AL, Cook KR, Belvin M, Dompe NA, Fawcett R, et al. Systematic generation of high-resolution deletion coverage of the Drosophila melanogaster genome. Nat Genet. 2004;36:288–292. [PubMed]
72. Warn RM, Magrath R. F-actin distribution during the cellularization of the Drosophila embryo visualized with FL-phalloidin. Exp Cell Res. 1983;143:103–114. [PubMed]

Articles from PLoS ONE are provided here courtesy of Public Library of Science