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Mice homozygous for mutations in Dact1 (Dpr/Frodo) phenocopy human malformations involving the spine, genitourinary system, and distal digestive tract. We trace this phenotype to disrupted germ layer morphogenesis at the primitive streak (PS). Remarkably, heterozygous mutation of Vangl2, a transmembrane component of the Planar Cell Polarity (PCP) pathway, rescues recessive Dact1 phenotypes, whereas loss of Dact1 reciprocally rescues semidominant Vangl2 phenotypes. We show that Dact1, an intracellular protein, forms a complex with Vangl2. In Dact1 mutants, Vangl2 is increased at the PS where cells ordinarily undergo an epithelial-mesenchymal transition. This is associated with abnormal E-cadherin distribution and changes in biochemical measures of the PCP pathway. We conclude that Dact1 contributes to morphogenesis at the PS by regulating Vangl2 upstream of cell adhesion and the PCP pathway.
Multiple developmental events occur at or within close proximity to the primitive streak (PS) in the posterior embryo. These include epithelial-mesenchymal transition (EMT) associated with specification of primary germ layers, ventral closure of endoderm to form hindgut, medial-lateral division of mesoderm, posterior elongation of the notochord, segment formation, and dorsal closure of neuroectoderm to form the neural tube. Planar Cell Polarity (PCP) and Wnt/β-catenin signaling are both involved in these processes1-4.
Vangl2 (Van Gogh-like/Strabismus) is a four-pass-transmembrane protein that plays a major role in the PCP pathway. By establishing asymmetric localization of both membrane and cytoplasmic components, this pathway regulates cell polarity and movements, particularly convergent-extension (CE) movements that shape germ layer derivatives shortly after gastrulation at the PS5. Vangl proteins directly interact with the intracellular protein Dishevelled (Dvl), a central component of both the PCP and Wnt/ß-catenin signaling pathways6. The Wnt/β-catenin pathway is mechanistically distinct from PCP; it determines cell decisions by regulating transcriptional activity of target genes downstream of post-translational stabilization of the β-catenin protein7.
Mice with mutations affecting each of these pathways have phenotypes linked to events in the PS region. For example, mutations in Wnt3a, a posterior patterning ligand that activates the Wnt/β-catenin pathway, cause posterior truncation stemming from defective mesoderm specification1. Mutations in Vangl family members that diminish PCP activity cause neural tube defects traced to defective cell movements in the neuroectoderm2. Despite established roles in both these pathways in other systems, Dvl mutations have so far been linked only to PCP phenotypes in mice8.
Dact (Dapper/Frodo) proteins bind Dvl and have been shown to modulate several signaling pathways, including Wnt/β-catenin signaling9-13. By studying an engineered mutation in mouse Dact1, we have discovered strong and reciprocal genetic interactions with Vangl2. Biochemical and embryonic analyses reveal that this unusual genetic relationship reflects a role for Dact1 in post-translational regulation of Vangl2 at the PS, upstream of cell adhesion and PCP signaling.
We genetically engineered an allelic series at the mouse Dact1 locus including two equally severe alleles deduced to be nulls on molecular and biochemical grounds (Supplementary Fig 1). One allele (Dact1neoΔ) was backcrossed for more than ten generations to the C57BL/6 isogenic mouse strain for use in this study; these homozygotes are hereafter referred to as Dact1 mutants.
Dact1 mutants are born at near Mendelian ratios (Supplementary Table 1a), but with rare exceptions die within a day of birth. These neonates have a short tail, no anus, no urinary outlet, nor external genitalia (Fig 1a-d). Internally, the vast majority have blind-ended colons (Fig 1e-f) and no bladder (Fig 1g-h, Supplementary Table 1b). Ureters are present but connect at the midline or fuse with the reproductive ducts, while the kidneys are invariably hydronephrotic (Fig 1h). The kidneys also display variable developmental malformations ranging from fusion at the midline to complete agenesis (Fig 1h, Supplementary Table 1c). Rare mutants (<1%) that survive postnatally nonetheless have non-lethal genitourinary and digestive tract abnormalities evident upon laparotomy (Fig 1i-k). Gonads of mutants of both sexes are typically present and grossly normal (Fig 1h).
In addition to genitourinary and gastrointestinal phenotypes, most (~90%) Dact1 mutants are immediately distinguishable from littermates by virtue of segmental truncation (Fig 1a-b; Supplementary Table 1d). Skeletal analysis reveals segmental loss that is most commonly (73%) restricted to the tail (Fig 1l-m; o-p). A smaller percentage (17%) has truncations extending into sacral and lumbar regions (Fig 1n, q); these are rarely accompanied by malformations of the pelvis and hindlimbs, including sirenomelia (Fig 1r). Most severely truncated mutants have spina bifida (13% of total; Fig 1s). Although there are usually a few smaller malformed vertebrae immediately anterior to the segmental truncation, all other vertebrae and ribs are of normal size, morphology, and identity (Fig 1p-q). Since segmentation in vertebrates proceeds from anterior to posterior15, the striking lack of anterior segment abnormalities in Dact1 mutants suggests segmentation failure restricted to late developmental stages, as opposed to a more general disruption of this process16,17.
The earliest developmental differences we detect in Dact1 mutants occur at embryonic day (E) 8.25, shortly after segmentation begins when the embryo has 4-7 newly formed somites15. Unstained wild type and mutant embryos are indistinguishable anteriorly (Fig 2a-b), and whole mount mRNA in situ hybridization (WISH) using an Uncx4.1 probe that marks the posterior compartment of each segment16, demonstrates that somites are normal (Fig 2a-b insets) at this stage. Nonetheless, Dact1 mutants are misshapen posteriorly in the region of the PS. Viewed dorsally, the wild type embryo has a rounded posterior contour (Fig 2a) whereas Dact1 mutants are slightly spade shaped: widening abnormally before tapering to a more pointed tip (Fig 2b asterisk). As morphological differences in Dact1 mutants are confined to the posterior, we quantified them by measuring Length-Width Ratio (LWR) specifically in this region (“Posterior LWR”; Methods). Posterior LWR at the 6-7 somite stage is significantly reduced in Dact1 mutant embryos compared to wild type (1.57 ± 0.05 vs. 1.85 ± 0.04, p = 0.0008) (Fig 2c). We also detected a significant reduction compared to wild type in the Posterior LWR of Vangl2Lp/+ embryos (1.67 ± 0.04 vs. 1.85 ± 0.04, p = 0.0096) (Fig 2c), which are heterozygous for a semidominant allele in Vangl218. Consistent with a prior report3, using LWR based on the whole embryo (“whole embryo LWR”; Methods), we detected no significant differences between wild type (9.42 ± 0.23) and Vangl2Lp/+ (9.05 ± 0.36; p = 0.4) at the 6-7 somite stage, nor between wild type and Dact1 mutants (9.48 ± 0.43; p = 0.9) (Fig 2d). Since CE movements in the posterior embryo have been shown to be affected in Vangl2Lp/+ embryos at this stage4, our findings suggest that Posterior LWR reflects cell movements within this embryonic region, and that these are disrupted in Dact1 mutants.
We next used a panel of WISH markers to assess morphology of individual tissues in this region. Viewed from either the ventral or lateral aspect, WISH for Shh shows that the presumptive notochord domain19 is broader in Dact1 mutants and does not extend as far posteriorly beyond the last-formed somite (labeled by Uncx4.1 WISH) (Fig 2e-h). There are also differences in morphology of the posterior endoderm, which like the presumptive notochord domain does not extend as far posteriorly and is delayed in folding ventrally to form the hindgut diverticulum (Fig 2g-h). Presomitic mesoderm labeled with Dll1 is normal in volume but is redistributed around the shortened axial and ventral structures (Fig 2i-j). Unlike the shortened axial mesoderm and endoderm, the ectoderm in Dact1 mutants extends to the posterior tip of the embryo, even in mutants where ventral defects are severe (Fig 2i-j arrows).
Consistent with these WISH data, cross section at the PS reveals that all three germ layers are present in the posterior Dact1 mutant embryo at the 6 somite stage, but there is a notable divergence from wild type morphology. The endoderm is open ventrally and fails to form a tubular hindgut with columnar epithelium (Fig 2k-l). Ectoderm morphology is variable but is often 1 to 2 cells thicker apical-basally, and is more acutely folded (Fig 2k-l insets & asterisk). Rates of proliferation and cell death are not significantly different in this region even in mutants with severely affected morphology (Supplementary Fig 2).
To investigate how these early morphological defects progress, we examined the development of germ layer derivatives at later stages. At E9.5, presomitic mesoderm expressing Dll1 continues to extend fully posteriorly in mutants, as does the overlying ectoderm (Fig 2m-n). However, axial structures that normally separate left from right presomitic (paraxial) mesoderm terminate more anteriorly, such that this tissue assumes an abnormal Y-instead of a U-shape when viewed dorsally (Fig 2o-p).
The posterior segments that are frequently missing in Dact1 mutants are generated only after E9.5 from the presomitic mesoderm (PSM) located in the tail bud15. Concordantly, Uncx4.1 WISH reveals segmental defects only after E9.5 and only in the most recently formed somites (Fig 2q-r). Segmentation is governed in part by the somitogenesis cycle, a regular oscillation of gene expression in the PSM, and some mutations that cause segmental loss disrupt this cycle throughout development20. We tested whether Dact1 mutants have disruptions in the somitogenesis cycle at late stages by examining expression of well-established somitogenesis genes such as Lfng16,20. Expression of Lfng and other somitogenesis cycle markers was disrupted in Dact1 mutants by E10.5 (Fig 2s-t; Supplementary Table 2). However, these somitogenesis cycle defects never occurred before E10 and never in isolation: mutant tail buds by this stage invariably displayed extensive anatomical disorganization and evidence of histolysis including absence of the tail gut (posterior endoderm), severe shortening of the notochord, and pockets of pooled blood and serous fluid (Fig 2u-x; Supplementary Table 2).
Taken together, these embryological data suggest that the Dact1 mutant phenotype arises from a primary defect in germ layer morphogenesis at the PS; segmental truncations in these mutants are associated with failed somitogenesis occurring in the context of tail bud disorganization and deterioration at later stages.
Work in other systems has suggested that Dact1 primarily modulates Wnt/β-catenin signaling9,10,12,13. We accordingly asked whether Wnt/β-catenin pathway defects underlie the earliest observable Dact1 mutant phenotypes in the posterior embryo. We measured Wnt/β-catenin target mRNA levels by Quantitative Reverse Transcriptase PCR (QPCR) at the stage when morphological differences are first detected in Dact1 mutants (5-7 somites). We validated this assay using previously studied signaling mutants4,17 and the established Wnt/β-catenin targets, Dll1 and Axin221. Levels of both these targets were significantly reduced in posterior tissues from Wnt3a null embryos compared to control littermates (% of average wild type for Dll1: 16 ± 2 vs. 100 ± 10; p<0.0001, for Axin2: 42 ± 7 vs. 100 ± 14; p=0.004) (Fig 3a-b). Moreover, levels of these targets were not significantly different in posterior tissues from heterozygotes for the semidominant PCP signaling mutant Vangl2Lp (% of average wild type for Dll1: 121 ± 11 vs. 100 ± 9; p=0.2, for Axin2: 77 ± 11 vs. 100 ± 20; p = 0.3) (Fig 3c-d). Dact1 mutant posterior tissues showed no significant differences in these Wnt/β-catenin target gene levels compared to controls (% of average wild type for Dll1: 95 ± 8 vs. 100 ± 7; p = 0.6, for Axin2: 85 ± 17 vs. 100 ± 15; p = 0.5) (Fig 3e-f). Similarly, we measured levels of activated β-catenin protein at E9 by immunoblot with dephospho-specific β-catenin antibody (mAb 8E7)22; there were no significant differences compared to controls (% of average wild type = 81 ± 8 vs. 100 ± 10; p = 0.2) (Fig 3g-h). Finally, when assessed by WISH, expression of the posterior Wnt/β-catenin signaling targets Dll1 and Brachyury (T) were not significantly reduced in Dact1 mutant embryos (Fig 2i-j, m-p; Supplementary Fig 3a-b). We also detected no differences in levels of the p120-catenin (Ctnnd1) or Dvl proteins (Supplementary Fig 3c-d), previously shown to be regulated by Dact family members in other contexts9,13,23.
Some of the phenotypes observed in Dact1 mutants, such as neural tube defects, broadening of the presumptive notochord domain, and differences in posterior LWR, resemble those known to result from PCP pathway disruptions4,24. Among several putative intracellular effectors, PCP signaling is linked to regulation of two kinases: Rho associated kinase4 and c-Jun N-terminal Kinase (JNK)5. We tested whether activities of these kinases are altered in the Dact1 mutant posterior embryo. To assess Rho kinase activity we used immunoblotting with a phospho-specific antibody to measure amounts of its phosphorylated substrate, Mypt125. In E8 posterior embryo lysates from Dact1 mutants, levels of phosphorylated Mypt1 were significantly reduced compared to controls (% of average wild type = 69 ± 9 vs. 100 ± 8; p = 0.03) (Fig 3i-j). We measured activated JNK in posterior embryo lysates at E9 through direct phosphorylation of a GST-Jun fusion protein normalized against total JNK recovered in a pull-down assay26. Endogenous JNK activity was unambiguously increased in Dact1 mutant posterior embryos at this stage (% of average wild type = 258 ± 19 vs. 99 ± 13; p = 0.0005) (Fig 3k-l).
In summary, molecular, biochemical, and embryonic assays at early phenotypic stages do not support changes in Wnt/β-catenin signaling in Dact1 mutants; they instead indicate defects in the PCP pathway.
In mice, synergy with one copy of Vangl2Lp to cause neural tube defects is generally accepted as evidence that a genetic locus participates in the PCP pathway3. Because Dact1 mutants display a partially penetrant neural tube defect (spina bifida) and also have abnormalities in embryological and biochemical measures associated with PCP signaling, we predicted that mice homozygous for the Dact1 mutation and heterozygous for Vangl2Lp would display severe defects in neural tube closure.
Unexpectedly, mutations in Dact1 and Vangl2 mutually rescue each other, such that nearly all Dact1 mutant mice heterozygous for Vangl2Lp appear grossly normal and display neither Vangl2Lp semidominant nor Dact1 recessive phenotypes (Fig 4a-d). From a cross conducted in a 97% isogenic C57Bl/6 genetic background, approximately 80% (9/11) of Dact1-/-;Vangl2Lp/+ mice had normal genitourinary (GU) systems, normal gastrointestinal (GI) systems, no segmental truncation, and no neural tube defects, compared to Dact1-/-;Vangl2+/+ littermates of which 100% (11/11) had GU phenotypes, 90% (10/11) had GI phenotypes, >50% (6/11) had segmental truncation, and ~20% (2/11) had spina bifida (Fig 4e red vs. blue; Supplementary Table 3a). Vangl2 mutant-mediated rescue of the Dact1 mutant phenotype is not due to a molecular peculiarity of the Vangl2Lp allele because a very similar pattern of rescue is observed with an independently derived allele27, Vangl2Lp-m1Jus (Fig 4e green vs. yellow; Supplementary Table 3a). Conversely, whereas more than 80% of animals heterozygous for either Vangl2Lp or Vangl2Lp-m1Jus (5/6 & 8/10 respectively) display the characteristic semidominant curly tail (Looptail) phenotype, penetrance of this phenotype drops to <65% (11/17 & 9/22 respectively) when animals are heterozygous, and to ≤20% (1/10 & 3/15 respectively) when homozygous, for the Dact1 mutant allele (Fig 4f; Supplementary Table 3b). Nevertheless, although Dact1 loss rescues the semidominant Loop-tail phenotype, it does not rescue the recessive craniorachischesis phenotype of homozygous Vangl2 mutant embryos (Supplementary Fig 4).
To summarize, genetic experiments demonstrate that recessive Dact1 mutant phenotypes are abrogated by mutation of one Vangl2 allele, and conversely that semidominant Vangl2 mutant phenotypes are ameliorated by loss of Dact1. Failure to rescue the homozygous Vangl2 mutant phenotype demonstrates that a functional allele of Vangl2 is required for this reciprocal genetic interaction.
One mechanism whereby Dact1 could regulate Vangl2 is through physical interaction. We tested this hypothesis through a series of co-immunoprecipitation (coIP) and pull-down assays, results of which are schematically summarized in Figure 5a-c.
When co-expressed in human embryonic kidney (HEK 293) cells, the Vangl2 protein coIPs with Dact1 (Fig 5d). We determined the region of Dact1 responsible for this interaction through a panel of Dact1 deletion constructs. Loss of the C-terminal 88 amino acids (aa) of Dact1 almost completely eliminates association with Vangl2, and the residual interaction is abolished by deletion of an additional 62 aa (Fig 5d). Under identical conditions, the same panel of Dact1 constructs shows a different coIP pattern with Dvl2: Progressive C-terminal deletions of Dact1 reduce but do not eliminate association with Dvl2 until elimination of aa 311-778 (Fig 5e). The Dact1 PDZb caps a longer stretch of 28 highly conserved aa14, and so we made specific deletions to probe how this region compares to the immediately upstream 60 aa in coIPs with Vangl2 versus Dvl2. Deletion of the Dact1 C-terminal 28 aa has no effect on association with Vangl2 (Fig 5f), but reduces association with Dvl2 at least as much as larger deletions (Fig 5g). Conversely, internal deletion of the adjacent 60 aa has no effect on Dact1 association with Dvl2 (Fig 5g), but reduces association with Vangl2 similar to larger deletions (Fig 5f). Taken together these data strongly suggest that separate domains of Dact1 contribute to complex formation with Vangl2 versus Dvl2.
We similarly used a series of Dvl2 deletion constructs to probe whether different conserved regions of Dvl are responsible for associations with Dact1 versus Vangl2. Consistent with prior reports6,28, we found that the Dvl PDZ domain is the main contributor to the Dvl-Vangl2 interaction (Fig 5h). We also found that a “Dishevelled Specific” (DS) domain (Methods) contributes modestly to this interaction (Fig 5h). In contrast, using the same panel of Dvl2 constructs under identical conditions we found that deletion of the PDZ and DS domains reduces but does not eliminate the Dvl-Dact1 interaction (Fig 5i). Taken together, these coIP data strongly suggest that besides PDZ-b/PDZ binding12, a middle region of Dact1 also contributes to interactions with Dvl2 outside the PDZ domain, consistent with some prior reports9,10.
These experiments indicate that different domains contribute to associations between Dact1 and Dvl2 versus either of these proteins with Vangl2. In a final assay we asked whether Vangl2 can bind directly to Dact1 in the absence of Dvl proteins. Since Dvl proteins are specific to metazoans, we bacterially expressed and purified recombinant GST fusion proteins corresponding to the amino-and carboxy-terminal regions of Dact1 and asked whether they bind to full-length Vangl2 protein synthesized in a wheat germ extract. The C-terminal half of Dact1 binds specifically to Vangl2 in this Dvl-free system, supporting the conclusion that the Dact1-Vangl2 interaction is direct (Fig 5j).
By prior report, Vangl2 is expressed at low levels in the posterior endoderm and at higher levels in the neuroectoderm, which is contiguous with ectoderm in the PS region29,30. Dact1 is expressed in a potentially overlapping domain in the posterior ectoderm and mesoderm31. This suggests that Dact1 and Vangl2 might functionally interact in these tissues, particularly in the PS ectoderm.
Using WISH we confirmed that the mRNA distributions of Dact1 (Fig 6a-b) and Vangl2 (Fig 6c-d) overlap in PS ectoderm. As expected for a transmembrane protein and consistent with prior reports29, an affinity-purified antibody detects Vangl2 protein primarily on surfaces of epithelial cells in the PS ectoderm and endoderm, as well as more weakly on scattered surface subdomains of adjacent mesenchymal cells (Fig 6e inset; arrowheads). The adhesion protein E-cadherin shows a partially overlapping distribution with Vangl2 in all germ layers, but is concentrated at the apical and basal surfaces and is generally less apparent on the lateral membranes of ectoderm cells (Fig 6f-g inset).
In the PS ectoderm of Dact1 mutants, Vangl2 cell surface signal is significantly increased (Fig 6h; Supplementary Fig 5b; e). Moreover, cell surface E-cadherin is also significantly increased and colocalizes with the Vangl2 signal, no longer displaying enrichment on the apical-basal vs. lateral cell surfaces (Fig 6i-j; Supplementary Fig 5b; f). This is a post-translational effect, as levels of both the Vangl2 and E-cadherin mRNAs are not altered (Supplementary Fig 6a-b). In these mutants, cells with high Vangl2 and E-cadherin form a bulge at the position of the PS where EMT normally occurs (Fig 6j dotted lines).
Prior reports suggest that the Vangl2Lp mutation alters the ability of mutant Vangl2 protein to stably accumulate at the membrane, especially asymmetrically or at points of cell contact18,32,33. Consistent with this, we find that in Vangl2Lp/+ embryos, Vangl2 protein remains detectable in cells where the wild type protein is typically expressed, but the membrane signal is significantly reduced compared to wild type (Fig 6k; Supplementary Fig 5c; e). Interestingly, E-cadherin is also mislocalized in these cells: a diffuse cytoplasmic signal appears that is absent from wild type controls (Fig 6l). Nevertheless, some apical-basal enrichment of E-cadherin remains evident (Fig 6l inset), and levels on the lateral edges of PS ectoderm cells are as low as in wild type (Supplementary Fig 5c; f).
The PS ectoderm in Dact1-/-;Vangl2Lp/+ combination mutants has Vangl2 cell surface staining intermediate between the high signal detected in Dact1 mutants and the low signal detected in Vangl2Lp/+ embryos, such that levels are not significantly different from wild type controls (Fig 6n inset; Supplementary Fig 5d; e). In contrast to Dact1 single mutants, Dact1-/-;Vangl2Lp/+ combination mutants also have normal surface levels and a more normal apical-basal distribution of E-cadherin in PS ectoderm cells (Supplementary Fig 5f; Fig 6o inset). Finally, the bulge of cells with high Vangl2 and E-cadherin found at the PS in Dact1 single mutants is absent from combination mutants (Fig 6p dotted lines).
To summarize, loss of Dact1 leads to increased Vangl2 and E-cadherin in the PS ectoderm where cells normally undergo EMT. In Vangl2Lp heterozygotes, there is partial loss of membrane Vangl2 signal; this most likely reflects the absence of surface-destabilized mutant protein made from the Loop-tail allele32. Compared to Dact1 mutants, Dact1-/-;Vangl2Lp/+ combination mutant embryos have partially restored cell surface Vangl2 levels, E-cadherin distribution, and PS morphology.
The phenotypic spectrum in Dact1 mutant mice is reminiscent of a similar spectrum of posterior malformations in humans34. Etiologies previously proposed to explain all or part of this spectrum include vascular-steal35, persistence of the embryonic cloaca36, and defects in posterior mesoderm formation37. Our findings suggest that this malformation spectrum may first originate in disturbed morphogenetic movements at the PS in the early embryo.
Several morphogenetic processes take place in close spatial and temporal proximity in the posterior embryo, each of which is likely to require dynamic regulation and polarized activities of Vangl2, the PCP pathway, and adhesive proteins. The first of these to occur is EMT at the PS, where both Dact1 and Vangl2 are expressed but where neither protein has a prior established role. Our data suggest that defective EMT is the primary defect in Dact1 mutants. Perhaps all other disrupted morphogenesis in these mutants occurs secondarily, for example because of decreased generation of mesoderm and endoderm precursors via EMT. Nonetheless we cannot rule out additional requirements for Dact1 alongside Vangl2 in spatially and temporally adjacent morphogenetic events, including CE movements that elongate and narrow axial mesoderm, mesenchymal-epithelial transition of endoderm precursors, or polarity and cell movements that fold and extend the hindgut.
Wnt/β-catenin signaling and E-cadherin negatively regulate each other at the PS, such that high E-cadherin reduces Wnt/β-catenin signal transduction in cells undergoing EMT38, and Wnt/β-catenin signaling reciprocally negatively regulates E-cadherin transcription39. We have observed no statistically significant alterations in Wnt/β-catenin signaling or in levels of E-cadherin mRNA in early Dact1 mutant embryos. Instead the E-cadherin protein is abnormally redistributed at early stages, whereas Wnt/β-catenin signaling reductions occur only much later in morphologically disrupted tail buds where they might contribute to somitogenesis failure specific to late-forming posterior segments (Supplementary Fig 6c-h)40. In any case, the rescue of all embryonic Dact1 mutant phenotypes by concurrent mutation of Vangl2 powerfully demonstrates that any E-cadherin or Wnt/β-catenin effects contributing to these phenotypes must occur downstream of Vangl2-dependent events.
We have discovered that a developmentally crucial function of Dact1 is regulation of Vangl2 at the PS. Morphogenetic abnormalities in the PS region of Dact1 mutant embryos, while partly resembling those caused by PCP pathway reduction4, are unique in that they are associated with decreased phosphorylation of the myosin binding subunit of myosin phosphatase (Mypt1), but increased JNK activity. This agrees with evidence that modulations in Rho-and Jun-kinase activities reflect separate pathways downstream of PCP4, and that either abnormal gain or loss of upstream PCP components can cause similar disruptions in cell polarity, cytoskeletal dynamics, and CE movements41-44. Interestingly, other PCP phenotypes, such as inner ear and cardiac malformations18,45, are not evident in Dact1 mutants (M. Montcouquiol, D.A.F., B.N.R.C., data not shown).
We propose that complex formation between the Dact1 and Vangl2 proteins is a crucial step in a novel Vangl2 regulatory pathway operating during EMT at the PS. Candidate cellular processes that might be involved include trafficking of Vangl2 to the membrane, endocytosis, subcellular sequestration, or degradation. This will be clarified by identifying additional components of this pathway through further biochemical, cellular, embryonic, and genetic experimentation.
Approximately 7 kb of Dact1 genomic DNA from the 129/Sv mouse strain was inserted into pGKneoF2L2DTA246 to create the Dact1 targeting vector (Supplementary Fig 1). Correct targeting through homologous recombination in ES cells was confirmed by Southern blot and PCR. Mice carrying the targeted allele were created using standard embryo manipulation and chimera breeding techniques. An allelic series at the Dact1 locus was created by crossing to the EIIaCre (The Jackson Laboratory, Bar Harbor, ME) and FLPe transgenic mouse strains in order to excise loxP-flanked and FRT-flanked sequences respectively. Genotyping was performed by genomic PCR using allele-specific primers: The primers Dact1intron1 and Dact1intron2 (See Supplementary Table 4 for this and all other primer sequences) are separated by 689 bases of genomic sequence in wild type, but only 190 bases in the excised (mutant) allele; amplifying a mutant-specific PCR product of 243 bases. The primers Dact1exon2 (near start exon 2) and Dact1intron2 (near the start of intron 2) are both within the floxed region; amplifying a wild type-specific PCR product of 330 bases. Amplification parameters for wild type: 30 cycles X (95°C 30 seconds, 52°C 30 seconds, 72°C 30 seconds); for mutant: 38 cycles X (95°C 30 seconds, 57°C 30 seconds, 72°C 30 seconds).
The Dact1 antibody was created by injecting rabbits with a peptide corresponding to aa 373-386 (coded within exon 4), followed by affinity purification. It is available from AbD Serotec.
Whole Embryo Length to Width Ratio (LWR): Whole embryo length (L) was the average distance along a straight line to the posterior tip of the embryo from the anterior tips of the right and left head folds. Whole embryo width (W) was the distance between the lateral edges of the left and right somites positioned in the middle of the anterior-posterior axis (L/2). LWR was calculated as L/W.
Posterior Length to Width Ratio (LWR): Posterior length (L) was the average distance along a straight line to the posterior tip of the embryo from the posterior edges of the most posterior (last formed) left and right somites. Posterior embryo width (W) was the widest lateral distance across the embryo (perpendicular to L) in the region corresponding to L (posterior to the last formed somite). LWR was calculated as L/W.
To measure proliferation and apoptosis, embryos were sectioned and stained for phalloidin, Hoescht 33258, and phospho-histone-H3 (Millipore) or active caspase-3 (BD Biosciences), respectively. Staining was visualized on a Nikon C1si Spectral Confocal microscope. A single confocal plane from each 20μm section was used to avoid double counting of cells. Graphs show the average percent proliferative or apoptotic cells across all sections (n = 2 embryos for each genotype, 5 sections per embryo) from the same genotype. There were no significant differences between mutants and controls for all these measures.
As described14 with the following modifications: Samples were embryonic tissues posterior to the last-formed somite. 0.5-1μg of total RNA was used for cDNA synthesis. Primers: QAxin2F, QAxin2R, QDll1F, QDll1R, QVangl2F, QVangl2R, QLacZF, QLacZR and for E-cadherin as described47.
Embryonic tissues posterior to the last-formed somite were homogenized in 100ul buffer and assayed as described26.
Association assays were performed essentially as described48. GST pull downs were in PBS + 0.1% Triton-X-100 (Roche), 0.1% insulin. Binding was at 4°C for 30 minutes, followed by 3 X 5 minute washes in binding buffer at 4°C. 35S-labelled in vitro translated proteins were synthesized in the TNT coupled wheat germ extract system (Promega). cDNAs were obtained commercially or by RT-PCR from wild type mouse total RNA. Expression and deletion plasmids were constructed using standard restriction digest and/or PCR techniques, and confirmed by sequencing. For Dvl2 the DS (pfam02377; aa 160-232), PDZ (cd00992; aa 265-352) and combined deletions are precise inverse PCR-mediated deletions of these domains as defined on the NCBI Uniprot website. The b (basic) domain is a conserved Arginine/Lysine-rich stretch located just upstream of the PDZ49, corresponds to aa 231-249 of mouse Dvl2, and is therefore distinct from the DS domain. Commercial antibodies (sources): Activated ß-Catenin “ABC” (Millipore)22, Vangl2, Dvl1, Dvl3, HA, FLAG (Santa Cruz Biotech), Dvl2 (Cell Signaling Technology), p120catenin (BD Biosciences), α-tubulin (Sigma-Aldrich), Phospho-Mypt (T696) (Millipore), Total Mypt1 (BD Biosciences).
Genotyping for crosses was performed by Crp microsatellite PCR50. Genotypes of all combination mutant (experimental) and control littermates was verified by genomic PCR amplification and sequencing of alleles. Primers for PCR: Vangl2LpF and Vangl2LpR; for sequencing: Vangl2Lpseq.
Genotyping was performed by allele-specific PCR using primers homologous to the wild type versus the point mutant allele (Supplementary Fig 7). We used the primer pair Lp-m1JusWTF and Lp-m1JusWTR to amplify a 402 base pair wild type allele product using the following parameters: 30 cycles X (95°C 30 seconds, 68°C 30 seconds, 72°C 1 minute). We used the primer pair Lp-m1JusWT F and Lpm1JusMutR to amplify a 402 base pair mutant allele product using the following parameters: 30 cycles X (95°C 30 seconds, 62°C 30seconds, 72°C 1 minute).
Genotyping was performed by genomic PCR with allele-specific primers. Primers and parameters for the wild type allele were as recommended by the supplier (The Jackson Laboratory). We used primer pair Wnt3aneo and Wnt3aintron2 to amplify a Wnt3aneo-specific 386 base pair product using parameters: 35 cycles X (95°C 30 seconds, 65°C 30 seconds, 72°C 1 minute).
Embryos were dissected in PBS, fixed in 4% paraformaldehyde for 1 hour at room temperature (RT), and washed in PBS. For embedding, embryos were incubated in 30% glucose in PBS at 4°C overnight, equilibrated with equal parts 30% glucose and O.C.T. compound (Tissue-Tek) for 2 hours on ice, then embedded in 30% glucose and O.C.T. compound. Embryos were cryosectioned (20μm) at -16°C. Sections were dried at RT, washed 2x in PBS for 5 minutes, blocked for 1.5 hour at RT using 10% heat inactivated goat serum, 1% BSA in PBS, then incubated in primary antibody overnight at 4°C. Rabbit Vangl2 antibody18 and Mouse E-cadherin antibody (BD Biosciences) were diluted 1:500 in 1% heat inactivated goat serum, 1% BSA in PBS. Sections were washed 5× 10 min in PBS, blocked, and incubated in anti-rabbit alexa fluor 488 and anti-mouse alexa fluor 568 (Molecular Probes) diluted 1:250 overnight at 4°C. Sections were washed 5×10 min in PBS, mounted in Mowiol and imaged via confocal microscopy under identical non-saturating illumination conditions.
Signal intensity (grey scale) was measured using ImageJ software (NIH), across a straight line drawn parallel to the apical surface of the PS ectoderm and bisecting 5 adjacent cells. Pixel intensity was normalized to the lowest value along the entire line, which was set to 0 (background). For comparisons of cell surface intensity between cells, the 3 highest adjacent values corresponding to the two lateral cell surfaces (6 values total/cell) were averaged and plotted.
All quantitative data were analyzed using Prism software (Graphpad). Significance was determined by parametric unpaired two-tailed t tests. In all cluster graphs, mean values are plotted as a horizontal line; numerical values for the mean, standard error, and p-value are reported in the corresponding Results text.
We thank all members of the Cheyette laboratory for thoughtful input and assistance with mouse husbandry and genetics. Eric P. Fox provided technical expertise for creation of the Dact1 targeting construct, starting from the pGKneoF2L2DTA2 vector donated by Philippe Soriano. ES cell manipulation and chimera production were accomplished at the University of Washington Transgenic Resources Program. Uta Grieshammer of the UCSF Department of Anatomy provided expert assistance with neonatal genitourinary phenotyping. Confocal microscopy was accomplished at the Nikon Imaging Center at UCSF/QB3, with advice from Kurt Thorn. Susan Dymecki provided the FLPe transgenic mouse line, Andrew McMahon the Wnt3a mutant mouse line, and Stefano Piccolo the BAT-gal line. Thomas Gridley provided probes for Uncx4.1 and Dll1. Mireille Montcouquiol provided affinity-purified Vangl2 antibody. Anthony Wynshaw-Boris provided helpful comments on the final manuscript. BNRC gratefully acknowledges support from NIH R01HD055300, the Sandler Foundation, the UCSF Academic Senate Committee on Research, and the UCSF Center for Neurobiology and Psychiatry. R.S. is a recipient of a predoctoral fellowship from the California Institute of Regenerative Medicine. D.A.F. received support from the MSTP at Washington University St. Louis.
AUTHOR CONTRIBUTIONS R.S. contributed gene expression, QPCR (Wnt signaling targets), most embryological analyses, confocal microscopy, and genetics. S.K. contributed antigen synthesis, antibody characterization, Western blots, kinase assays, coIPs, pull-downs, and associated plasmid constructs. D.A.F. contributed skeletal and somitogenic analyses, BAT-gal WISH, and genetics including the initial Vangl2Lp cross. B.N.R.C. designed the Dact1 targeting construct in the laboratory of R.T.M. at the UW. The experiments of R.S., S.K., and D.A.F. were performed at UCSF in the laboratory of B.N.R.C., who supervised this research and wrote the text with feedback from all authors.