Left-right asymmetry in vertebrates is initiated in an early embryonic structure called the ventral node in human and mouse, and the gastrocoel roof plate (GRP) in the frog. Within these structures, each epithelial cell bears a single motile cilium, and the concerted beating of these cilia produces a leftward fluid flow that is required to initiate left-right asymmetric gene expression. The leftward fluid flow is thought to result from the posterior tilt of the cilia, which protrude from near the posterior portion of each cell's apical surface. The cells, therefore, display a morphological planar polarization. Planar cell polarity (PCP) is manifested as the coordinated, polarized orientation of cells within epithelial sheets, or as directional cell migration and intercalation during convergent extension. A set of evolutionarily conserved proteins regulates PCP. Here, we provide evidence that vertebrate PCP proteins regulate planar polarity in the mouse ventral node and in the Xenopus gastrocoel roof plate. Asymmetric anterior localization of VANGL1 and PRICKLE2 (PK2) in mouse ventral node cells indicates that these cells are planar polarized by a conserved molecular mechanism. A weakly penetrant Vangl1 mutant phenotype suggests that compromised Vangl1 function may be associated with left-right laterality defects. Stronger functional evidence comes from the Xenopus GRP, where we show that perturbation of VANGL2 protein function disrupts the posterior localization of motile cilia that is required for leftward fluid flow, and causes aberrant expression of the left side-specific gene Nodal. The observation of anterior-posterior PCP in the mouse and in Xenopus embryonic organizers reflects a strong evolutionary conservation of this mechanism that is important for body plan determination.
Citation: Antic D, Stubbs JL, Suyama K, Kintner C, Scott MP, Axelrod JD (2010) Planar Cell Polarity Enables Posterior Localization of Nodal Cilia and Left-Right Axis Determination during Mouse and Xenopus Embryogenesis. PLoS ONE 5(2): e8999. doi:10.1371/journal.pone.0008999
Editor: Bruce Riley, Texas A&M University, United States of America
Received: December 16, 2009; Accepted: January 5, 2010; Published: February 2, 2010
Copyright: © 2010 Antic et al. This is an open-access article distributed under the terms of the Creative Commons Attribution License, which permits unrestricted use, distribution, and reproduction in any medium, provided the original author and source are credited.
Funding: This work was supported by R01 GM059823 (J.D.A.), by RO1 GM076507 (C.K.) and by the Howard Hughes Medical Institute. M.P.S. is an Investigator of the H.H.M.I. The funders had no role in study design, data collection and analysis, decision to publish, or preparation of the manuscript.
Competing interests: The authors have declared that no competing interests exist.
In the mouse, left-right asymmetry has been proposed to be controlled by fluid flow in the node propelled by clockwise movement of motile nodal cilia –. Leftward nodal flow depends on positioning of motile cilia at the posterior sides of nodal cells, causing an asymmetric stroke that produces the directional movement of the nodal fluid , . This flow begins at the 1 to 2 somite stage . Both mechanical effects of flow, and flow-dependent leftward transport of signaling molecules, have been proposed to set in motion asymmetric gene expression patterns that establish the laterality of subsequently developing structures –.
The asymmetric signal in the mouse ventral node initiates Nodal and Lefty signaling on the left side of the node and in the left lateral plate mesoderm (LPM) , . Nodal then induces expression of the homeobox gene Pitx2 that regulates asymmetric heart, gut, and lung morphogenesis , . While left-sided expression of Lefty and Nodal is transient, asymmetric expression of Pitx2 in LPM is maintained until E8.5 (8–9 somite stage) . Later in development, at stages E9.5 and E10.5, asymmetric distribution of Pitx2 is observed on the left side of the heart, foregut primordia, and lung buds , . In mutants with L-R asymmetry defects, such as iv/iv embryos, the expression of Pitx2 is either reversed, bilateral, or absent , .
In Xenopus, the gastrocoel roof plate (GRP) is homologous to the mouse ventral node and has a monociliated planar polarized epithelium. As in the mouse node, the cilia are motile, they are posteriorly located, and they rotate in a clockwise fashion thus generating leftward fluid flow. In both species, Inversin, Polycistin-2, and Dynein heavy chain proteins are important for ciliary structure, motility, and laterality determination , –. However, in neither system, is it known how the posterior localization and tilt of the motile cilia is established.
Planar polarization of cells is required in a variety of tissues during vertebrate development, and its disruption may lead to developmental anomalies including open neural tube defects, polycystic kidneys, conotruncal heart defects and deafness –. A number of genes, most first identified in Drosophila, are known to regulate PCP dependent processes. PCP signaling has been extensively studied in Drosophila using genetic and protein-localization approaches, revealing a tight link between asymmetric cortical distribution of PCP proteins and their PCP signaling functions –. Similar studies in mice showed that the mammalian PCP proteins Dishevelled (DVL2, DVL3), Frizzled (FZ3, FZ6), Van Gogh like (VANGL2; originally called Looptail), and PRICKLE2 (PK2) , ,– also localize asymmetrically in tissues that display planar polarity, such as the inner ear sensory epithelium. As in flies, PK2 and FZ6 accumulate on opposite sides of cells . These findings suggest that the PCP signaling mechanism in mammals is similar to that in flies , , . In both insects and vertebrates, PCP proteins influence cytoskeletal rearrangements that lead to specific orientation of morphologically polarized cells within epithelial sheets. Thus the PCP mechanism is an attractive candidate for determining the posterior localization and tilt of motile cilia in the mouse ventral node and in the Xenopus GRP.
We hypothesized that PCP may be required to position the nodal cilia in the posterior of each cell. If so, nodal cells must be polarized prior to the onset of nodal flow. To determine whether a conserved PCP signaling mechanism may establish PCP in the mouse ventral node, and if so, when this polarity is established, we used VANGL1, PK1, and PK2 antibodies to examine expression and localization of these proteins in early headfold stage embryos with 0 somites, prior to initiation of nodal flow, and in embryos with 1 to 2 somites, the time the nodal flow begins (Fig. 1). PK2 asymmetric distribution at anterior-posterior boundaries of central cells in the ventral node can be detected in very early headfold 0 somite embryos (Fig. 1A, C), presumably prior to the beginning of nodal flow. Asymmetric distribution of VANGL1 was also detected, but the earliest we detected it was later, at the 1 to 2 somite stage (Fig. 1B, C, E, F), the time when nodal flow begins. At this time, PK2 and VANGL1 colocalize. Both proteins appear to be at the anterior side of the cells, although mosaic studies will be needed to confirm this. Localization of these two PCP proteins in crescents is reminiscent of that seen in Drosophila tissues, and of PCP protein localization patterns in the vertebrate sensory epithelia of the inner ear , , , , . These observations reveal that the cells of the node exhibit molecular PCP along the anterior-posterior axis, and strongly suggest that the conserved PCP signaling system is engaged to polarize these cells along the anterior-posterior axis. The relevance of PK2 asymmetric distribution in crescents preceding that of VANGL1 is not clear, but might suggest that PK2 could be involved in establishing PCP while VANGL1 may be necessary to maintain it. We did not detect expression of PK1 in the ventral node (not shown), in agreement with reported in situ hybridization results .
(A–F) Localization of VL1 and PK2 proteins in the ventral node: PRICKLE2 is expressed in the node of 0 somite embryos (A, C red) prior to VANGL1, which is detected in node cells (E, F, green) of 1–2 somite embryos. VL1 and PK2 co-localize in node cells and form crescents pointed toward the anterior (F, yellow). Motile cilia can be visualized above the plane of VL1 or PK2 localization (not shown). Yellow letters mark anterior (A), posterior (P), Left (L) and right (R). As nodes were imaged from the ventral side, left side of the embryo is on the right side of each panel and right side of the embryo is on the left side of each panel.
To investigate the potential functional requirement for PCP signaling in vertebrate left-right asymmetry, we generated a Vangl1 mutant mouse using BayGenomics Vangl1 gene-trap ES cells, as has been done by another group  (Fig. S1). We similarly refer to the allele as Vangl1gt. In our animals of mixed genetic background, many Vangl1gt/gt homozygotes were viable and fertile as previously reported . Also as previously reported, we found that the two Vangl genes, Vangl1 and Vangl2, genetically interact to control PCP. Vangl1+/gt, Vangl2+/Lp doubly heterozygous mice had severe open neural tube defects as well as moderate PCP defects in cochlea (Fig. S1, S2), not present in either of the Vangl heterozygotes. In addition, we observed that at low penetrance, some homozygous Vangl1gt/gt mutants died as early embryos. The variable viability of our Vangl1gt/gt homozygous animals prompted us to carefully examine adult homozygotes for the expression of Vangl1-βGeo (the predicted mutant transcript that has β-Galactosidase-Neomycin fusion [βGeo] spliced after exon 3), Vangl1 WT mRNAs, and their corresponding proteins. Viable animals, homozygous for the gene-trap insertion, produced low but variable amounts of both Vangl1-βGeo and Vangl1 WT mRNAs and proteins (Fig. S3), suggesting that alternative splicing creates small amounts of functional Vangl1 transcripts and protein that are sufficient to suppress the homozygous null phenotype in the majority of individuals.
Analysis of animals from timed pregnancies revealed that 14% of Vangl1gt/gt homozygotes died early in development, between E9.5 and E10.5, and they displayed varying degrees of known PCP-related defects (Fig. 2). Each of five phenotypically mutant Vangl1gt/gt embryos we obtained at this stage had an open neural tube (Fig. 2), and the somites were narrow in the anterior-posterior direction and tended to be elongated medio-laterally compared to wild type, reminiscent of PCP dependent convergent extension defects (Fig, 3B', D' and not shown) , . Embryos with these phenotypes were never recovered among heterozygous siblings, or from crosses between wild-type, BL6 or 129Ola animals. In addition, despite advancing to the 20–25 somite stage and maintaining viability up to E9.5-E10 as judged by beating hearts at the time of isolation, each of the phenotypically mutant embryos failed to turn. The turning of mouse embryos is a process that converts the embryo from lordotic to fetal position at the 8- to 13-somite stage of development . Turning defects are often associated with aberrant L–R patterning in the mouse ventral node , , . Consistent with this interpretation, Pitx2 in two phenotypically mutant Vangl1gt/gt embryos isolated at E8.5 (Fig. 3) and E10 (not shown) was bilateral, with predominant expression on the right side of the embryo, consistent with aberrant L–R signaling. Normal left-sided expression of Pitx2 was observed in seven additional Vangl1gt/gt embryos with normal morphology that were obtained from these litters, as well as in all the embryos from five other litters from Vangl1gt/+ parents, from which we expect Mendelian ratios of Vangl1gt/gt homozygotes, although they were not genotyped. Therefore, abnormal Pitx2 expression appears to correlate closely with aberrant turning. While the abnormal turning and Pitx2 phenotypes, observed in a fraction of Vangl1gt/gt homozygous mutant mice, hint at a left-right lateralization function for Vangl1, the rarity of isolating phenotypically mutant embryos prevents us from doing a thorough analysis, and thus must be considered only suggestive of such a function. However, striking polarized distribution of VANGL1 and PK2 proteins in central node cells suggests that PCP signaling establishes anterior-posterior polarity and that this A–P polarity may be required for determining left-right asymmetry.
Vangl1+/gt heterozygous embryos are normal and they develop into viable, fertile adults. In contrast, ~14% of Vangl1gt/gt mutants die at E9.5–10.5. (A', B') Cranial (A') and dorsal (B') views of Vangl1gt/gt mutant embryos shown in A and B showing open neural tube defects. (B, B') One mutant and its heterozygous littermate were stained for VANGL1-βGEO fusion protein. Each of five phenotypically mutant Vangl1gt/gt homozygotes isolated at this stage failed to turn from lordotic to fetal position.
(A, B) Wild-type embryos with 7 somites (A, B, B') have Pitx2 expressed in the left lateral plate mesoderm (LPM). (C, D) A Vangl1gt/gt homozygous embryo with 8 somites has Pitx2 expressed bilaterally but predominant expression is in the right LPM. (D') Somites of the Vangl1gt/gt homozygous mutant are narrow and compressed in the anterior-posterior direction, in comparison to the wild-type embryo (B'). The mis-expression of Pitx2 and the turning defect suggest that Vangl1 might regulate L-R asymmetry establishment in the mouse ventral node. (B') and (D') are the boxed regions from (B) and (D) and are at the same magnification.
Because the low penetrance of obtaining phenotypically mutant Vangl1gt/gt homozygous embryos precluded analysis of mutant nodes, we chose to examine the role of PCP signaling in embryo lateralization in the homologous structure in Xenopus, the gastrocoel roof plate (GRP) –. In situ hybridization demonsrated that Vangl2 is the predominantly expressed Vang gene in the GRP (Fig. S4), while little or no Vangl1 expression could be detected (not shown). We have not been able to detect the localization of Xenopus VANGL2 protein in GRP cells, or in other tissues that are under control of a conserved PCP signaling mechanism based on strong functional evidence . Nonetheless, to determine whether PCP might contribute to the correct posterior placement of motile cilia in the GRP, we chose to knock down VANGL2 function using morpholinos. Morpholinos were injected at the eight-cell stage, and the affected cells traced with co-injected RFP, thereby knocking down Vangl2 expression within a subset of cells in both the deep and superficial mesoderm on the dorsal side. Injected embryos gastrulated normally, while the ciliated epithelium within the GRPs contained small cell clones with knocked down Vangl2 adjacent to wild-type, uninjected cells (Fig. 4). In GRP cells, motile cilia normally relocate from a predominantly middle to a predominantly posterior position, and this posterior positioning is required to produce leftward flow . In GRP cells with knocked down Vangl2, however, the distribution of cilia positioning is more central compared to the wild type distribution. This difference is statistically significant (Fig. 4A). As overexpression of PCP proteins is known to dominantly perturb polarity , we also disrupted PCP by overexpressing full-length Xenopus VANGL2 in the GRP by mRNA injection, and, similar to knockdown of Vangl2, we again observed a more central positioning of motile cilia compared to wild type (Fig. 4D–F). Together, these results indicate that PCP in the frog GRP regulates the posterior positioning of motile cilia required for leftward flow.
(A, D) A clone of cells in the GRP was generated by injecting one dorsal blastomere of 8-cell stage embryos with Vangl2 MO or a Vangl2 RNA, along with RFP RNA as a tracer or as a control. At stages 17/18, the dorsal half of the embryo was removed, fixed, and stained with antibodies directed to ZO-1 and acetylated–tubulin to mark cell boundaries and cilia, respectively. GRP cilia both inside (injected) and outside (uninjected) the clone were scored based on the location in GRP cells that were divided into three equal zones (anterior, middle and posterior). Shown are data from a minimum of 3 GRPs where 100–200 injected and uninjected cells were scored. Asterisks (* = p<0.05, ** = p<0.01.) represent p-values obtained using a two-tailed t-test. (B–C, E–F) Shown are confocal images of the GRP injected with the Vangl2 MO and RFP RNA (C), with Control MO and RFP RNA (B), with Vangl2 and RFP RNAs (F) or with RFP RNA alone (E). RFP (red) marks the position of the injected clone, cilia (green) are stained with the acetylated-tubulin antibody, and cell boundaries (blue) are stained with an antibody to ZO-1. Anterior is indicated by direction of the arrow in B, C, E, F.
To determine whether perturbing the posterior localization of motile cilia in the GRP affects left-right lateralization, we examined the expression of Xenopus nodal (Xnr1–Xenopus nodal related 1) mRNA in the Vangl2 morpholino treated embryos. Xnr1 is an early marker of lateralization that is normally expressed in the left lateral plate mesoderm (LPM) at late neurulation stage . In our experiments, 58% of Xenopus embryos treated with control morpholinos had normal expression of Xnr1, in the left LPM, with smaller fractions showing expression bilaterally, on the right, or not at all (Fig. 5). In contrast, in the Vangl2 morpholino treated embryos, lateralization was significantly impaired: only 9% showed Xnr1 expression in the left LPM, whereas the fractions with right sided, bilateral and absent expression were increased relative to controls. In the morpholino-treated embryos, the largest class (~53%) lacked expression of Xnr1. This result is similar to those previously reported upon knock-down of ciliary dynein heavy chain genes dnah9 and dnah5 or inhibition of the directional flow with methyl cellulose , . It contrasts with results obtained in mice, in which disruption of genes important for L–R determination results in increased right and bilateral but not absent expression of markers such as nodal or Pitx2 . It is important to note that our Vangl2 MO treated embryos did not display any signs of convergent extension defects, probably because Vangl2 was knocked-down in only approximately one of eight cells, and these intermingled with wild-type cells within the deep layer of the mesoderm during intercalation. Our results demonstrate that the PCP gene Vangl2 is required not only for posterior positioning of motile cilia in the GRP, but also for correct lateralization of Xenopus embryos.
(A) Xenopus embryos were injected with Vangl2 MO, or Control MO alone, targeting one dorsal blastomere at the 8-cell stage to generate a clone of injected cells within the GRP. At stages 20/21, embryos were fixed and probed by in-situ hybridization with an antisense Xenopus nodal-related1 (Xnr1) probe. Sidedness of staining was scored for at least 60 embryos for each condition. Data from one experiment are shown. (B–D) Shown are embryos injected with either Vangl2 or Control MOs and then probed with Xnr1 in-situ probe. Xnr1 staining is evident on the left (B) right (C) or both (D) sides of the midline. Black arrowheads indicate staining.
Our results from mouse and frog, taken together, suggest a conserved function for PCP in establishing L-R asymmetry in vertebrates. In mouse, at least two polarity proteins, VANGL1 and PK2, become asymmetrically distributed along the A–P axis in the node, most likely prior to L–R asymmetry determination, by localizing to anterior cortical domains in central node cells. We suggest that the very early establishment of PCP in the ventral node and GRP triggers the proper posterior localization of motile cilia that is required for efficient leftward nodal flow , , . Indeed, frog GRPs in which PCP is perturbed by knockdown or overexpression of Vangl2 show substantially less posterior bias of cilia positioning, and these embryos fail to correctly lateralize. Results of other studies predict that this would impair directional fluid flow produced by nodal cilia , .
Consistent with these results, in another report, Dishevelled (Dvl) compound mutant mice lacking 5 of 6 copies of the three Dvl genes also show L–R laterality defects, and motile cilia in the node are mislocalized . A DVL2-GFP showed that DVL2 protein, like VANGL1 and PK2, localizes to A–P cell boundaries in the ventral node, but to the posterior sides of cells , opposite to the apparent anterior localization of VANGL1 and PK2. DVL proteins are implicated in establishing the asymmetric cortical domains of PCP proteins , and have also been shown to be required for proper basal body and therefore cilia localization . It is not clear from these results in which capacity DVL proteins function in the ventral node. Based on the conserved localization of PK, VANG and DVL proteins in nodal epithelium, with PK2 and VANGL1 localized opposite to DVL2, one would predict that PCP proteins operate through asymmetric cortical domains to establish molecular asymmetry by a mechanism similar to that described in flies , , which would, in turn, affect placement of cilia and thus regulate morphologic planar polarity. The functional importance of VANG in regulating PCP in the Xenopus GRP also highlights the likelihood that the evolutionarily conserved mouse and frog nodal structures share this mechanistic feature required for embryonic lateralization .
The signals that operate upstream of the core PCP proteins to provide anterior-posterior directionality to the planar polarization of the ventral node or GRP are unknown. Similarly, the mechanism by which the anterior-posteriorly organized core proteins control the posterior localization of motile cilia is unknown. However, our results indicate that anterior-posterior PCP is important for establishment of vertebrate L–R asymmetry. The conservation of this mechanism in the mouse ventral node and the Xenopus GRP is reminiscent of anterior/posterior localization of PCP proteins in other organisms, and reflects deep conservation of molecular and, most likely, functional anterior/posterior polarization in the evolution of Chordates, from Ascidian notochord to zebrafish gastrula dorsal mesoderm, notochord, and neural keel cells –.
Generation of Vangl1 Deficient Mice
The ES cell line, XL802, containing the beta-Geo insertion in the third intron of the Vangl1 locus was purchased from BayGenomics (MMRRC at UC Davis, http://www.mmrrc.org/). The ES cells, genetically 129Ola, were injected into blastocysts isolated from C57BL/6 females (The Jaxon Laboratory) to generate chimeric males. Crosses between the chimeras and the C57BL/6 (Harlan, http://www.harlan.com/models/c57bl6.asp) females produced one F1 heterozygous male that was back-crossed with C57BL/6 females (Harlan) to generate a larger population of F2 heterozygous animals. Interbreeding of heterozygous animals produced subsequent generations of animals of mixed C57BL/6-129Ola background. Genotyping of 131 embryos extracted at E9.5 revealed that there were 35 (27%) Vangl1gt/gt homozygotes, 66 (50%) Vangl1+/gt heterozygotes, and 30 (23%) Vangl1+/+ homozygous embryos. From 35 Vangl1gt/gt homozygotes, only 5 (14%) had a mutant turning phenotype. All animals were maintained and bred according to Institutional Animal Care and Use guidelines under protocols approved by the Administrative Panel on Laboratory Animal Care (APLAC) at Stanford University.
Genotyping of Vangl1 Deficient Mice
The precise beta-Geo insertion site was mapped by PCR to nucleotide position 239 of the third intron. Based on the insertion site, the following primers were used for PCR based genotyping of the obtained animals: VL1-Ex3F primer (5′-CCATCCAGGCTCCTGCTGGAG-3′) was used as a “forward” primer for genotyping of the wild type (WT) and the beta-Geo containing Vangl1 locus, the VL1-Int3-2R primer (5′-CAGTCTCCAGATCTGTCCAGTCCCAAC-3′) was used as a “reverse” primer for the WT Vangl1 locus, and the BGeoR3 primer (5′-CGTGTCCTACAACACACACTCCAACC-3′) was used as a “reverse” primer for the Vangl1 knock-out locus. The PCR reactions were performed with Qiagen TaqMASTER Mix. The genotype of the obtained founder animals was further confirmed by Southern blotting (not shown).
RT-PCR for Vangl1-βGeo and Vangl1 WT mRNAs
Total RNA was isolated from adult cerebellum using Trisol reagent (Invitrogen). Vangl1-βGeo mRNA was detected using identical amounts of total RNA (300 ng) as template for each sample. The RT reaction was primed with BGeo-R1 primer (5′-GACAGTATCGGCCTCAGGAAGATCG-3′) and PCR reaction was carried out with Ex3F (5′-CCATCCAGGCTCCTGCTGGAG-3′) and BGeo-R1 primers. To detect Vangl1-WT mRNA, 300 ng of total RNA was used and the RT reaction was primed with an oligo-dT primer. 100 ng of each cDNA was used for the subsequent PCR reaction with 117-For (5′- CAGAGGGTCAGAAAAGTCTGTCACC-3′) and 996-Rev (5′-GCAATCATGGCTCGGGACTG-3′) primers. The specificity of the bands was confirmed with nested PCR using Ex3F and 943Rev (5′-CAGGCCAGCCATGTGCTTGG-3′) primers.
Crosses between Vangl1+/gt and Vangl2+/Lp (Lp/+) Animals
The Vangl2+/Lp animals were maintained in the mixed 129P2Ola/C57BL6 background. The animals had highly curled tails and females had imperforate vaginas. To obtain reproductively capable females, the Vangl2+/Lp males were out-crossed into the CD1 background for a maximum of two generations. Crosses between the two mouse strains were carried out with the F1 and F2 generation of Vangl1+/gt animals.
Cloning of the Mouse Vangl Genes
Vangl1 and Vangl2 genes were cloned by reverse-transcriptase-PCR from total RNA isolated from E18.5 CD-1 mouse embryos, using gene-specific primers designed according to the genomic sequence retrieved by the BLAT (BLAST-like Alignment Tool) program (University of California, Santa Cruz, http://genome.ucsc.edu/). The full-length cDNAs were cloned into eukaryotic expression vectors to generate either the YFP-tagged or untagged fusion constructs using the Invitrogen Gateway system (Carlsbad, CA).
Production and Dharacterization of VANGL1 Antisera
To produce antisera to mouse VANGL1 protein, a cDNA fragment encoding the 207 C-terminal amino acids of VANGL1 was subcloned into the pATH10 vector to generate TrpE fusion protein for rabbit and rat immunization. This region was also cloned into the pET28a vector to produce histidine-tagged VANGL1 fragment, which was used for affinity purification of the antiserum. Western blotting and immunohistochemistry were used to determine specificity of the VANGL1 antibody (Fig. S5). Human epithelial cervical cancer (HeLa) cells, obtained from ATCC (cell line CCL2), were transfected with the mammalian expression plasmid pDS (negative control), or with the pDS plasmid encoding the full-length untagged or YFP-tagged VANGL1 or VANGL2 proteins, using FuGENE (Roche, Indianapolis, IN). Protein lysates were made 24 hours after transfection in a hypotonic buffer containing 10 mM Tris, pH 7.5, 50 mM KCl, 5 mM EDTA, 1% Triton X100, and Roche complete protease inhibitors and were analyzed by Western blotting. In addition, VANGL1 purified antibody was used on blots to detect endogenous VANGL1 protein produced by inner ear sensory epithelial patches. The lysates were prepared from dissected sensory epithelia using hypotonic buffer and were analyzed by Western blotting either before or after endoglycosidaseF treatment (Roche, Indianapolis, IN).
Beta-Galactosidase Staining of Embryos
Mouse embryos were fixed in 4% paraformaldehyde in PBS, pH 7.4 for 20 minutes at 4°C, washed extensively in PBS, and stained with X-Gal (0.4 mg/ml X-gal, 10 mM potassium ferrocyanide, 10 mM potassium ferricyanide, 1 mM magnesium chloride in PBS) overnight at room temperature. After staining, embryos were fixed in 4% paraformaldehyde in PBS, pH 7.4 overnight at 4°C and were imaged as whole mounts (Leica MZFLIII dissecting scope).
Immunostaining of Node-Stage Embryos
Node stage embryos were dissected in ice-cold PBS and fixed in the ice-cold 4% paraformaldehyde in PBS, pH 7.4 for 2 hours at 4 C. Embryos were washed 4 times, 30 minutes per wash, in PBS at 4C and then incubated in BLOCK (PBS +0.1% TX100 +2%BSA) for 1 hour at room temperature. Staining was carried with the primary antibodies, diluted in BLOCK, for 3–4 hours at room temperature or over night at 4C and was followed by 3 washes, 30 minutes each wash, in PBS/0.1% TX100 (PBT). Secondary antibodies, diluted in BLOCK, were added and incubated for 1–2 hours at room temperature. Embryos were washed 3–4 times, 30 minutes each wash, in PBT and then mounted for confocal imaging.
Xenopus laevis Experiments
Xenopus embryos were obtained by in vitro fertilization using standard protocols. A synthetic Vangl2 mRNA (1–5 ng)  was injected into one dorsal animal blastomere of eight-cell stage Xenopus embryos . Cells derived from the injected blastomere were traced by co-injection of RNA encoding centrin fused to RFP (centrin-RFP) , or membrane-localized RFP . At stage 17, the gastrocoel roof plate (GRP) was dissected away from the embryo  in Danilchik's buffer +0.1% BSA and then held under a piece of coverglass for fixation in 4% paraformaldehyde in Phosphate Buffered Saline (PBS) for 1 hour on ice followed by dehydration in 100% ethanol. GRPs were rehydrated, washed with PBS/0.1% TritonX-100 (PBT), and blocked with PBT containing 10% heat-inactivated normal goat serum (PBT/HIGS) for at least one hour. GRPs were incubated with primary antibody in blocking solution overnight as follows: Rabbit anti-ZO-1 (Zymed 1:200), mouse monoclonal anti-acetylated tubulin (Sigma, 1:1000). After washing, GRPs were incubated overnight in Cy2, or Cy5 labeled Goat anti-IgG of the appropriate species (all used at 1:500, Jackson ImmunoResearch), washed in PBT and mounted in PVA/DABCO. Mounted embryos were imaged on a BioRad Radiance 2100 confocal mounted to a Zeiss inverted microscope using a 40× or 63× objective. Confocal images were false colored and z-stacks were compressed using NIH ImageJ. In some experiments, cilium location, based on centrin-RFP foci, was scored as being in the anterior, middle or posterior third of the cell in relation to the blastopore in each embryo. If centrin-RFP foci were not clearly evident, cilia were only scored if the entire cilium lay within a single one-third of the cell. In other experiments, cilium location was scored using acetylated tubulin, and cilia were only scored if the entire cilium lay within a single one-third of the cell. Data were gathered from 80–100 GRP cells marked with tracer as well as neighboring uninjected cells as a control, from at least 3 different embryos.
A morpholino (Genetools) directed against Vangl2 initiation codon, as described previously , or a standard control morpholino ,  was injected (20–30 ng; a concentration previously shown to produce a strong phenotype without toxicity) into one dorsal animal blastomere of eight-cell stage embryos in order to target the developing GRP . Cilia localization was analyzed as above for Vangl2 RNA injections. At stage 20–22, embryos were fixed and probed with an antisense probe directed against Xenopus nodal-related1 (Xnr1), to mark the lateral plate mesoderm, using standard in-situ hybridization protocols . Following labeling, experiments were blinded to the scorer and embryos were scored as having Xnr1 expression on the left side, right side, both sides or staining absent.
In this study, the following primary antibodies were used: rabbit anti-PK1, rabbit anti-PK2, rabbit and rat anti-VANGL1. These antibodies were generated in our labs. Commercially available antibodies used in this study were: mouse anti-spectrin (MAB1622, Chemicon, Temecula, CA), mouse anti-acetylated tubulin (T6793, Sigma, St. Louis, MO). Actin was stained with Alexa594-conjugated phalloidin (Invitrogen, CA). Secondary Antibodies coupled to Alexa 488, 594, or 633 dyes (Invitrogen) were used at 1:500 dilution.
Vangl1 mutant mice. (A, B) Map of the Vangl1 locus in Vangl1-deficient mice, and genotyping by PCR. (A) Diagrams of the Vangl1 genomic region containing a β-Geo insertion, the corresponding Vangl1-βGeo mRNA, and the resulting VANGL1-βGeo fusion protein. Remaining three exons and introns of the Vangl1 gene are not drawn but are indicated with an arrow after exon 4. Positions of primers used for PCR based genotyping are marked (> and <). The β-Geo gene, together with the splice acceptor (SA) site and the polyA tail, is inserted at position 239 of the 3rd intron in the Vangl1 locus of the XL802 ES cell line. The resulting VANGL1-βGeo fusion protein contains 70 N-terminal amino acids of the VANGL1 protein, and lacks all the trans-membrane domains (TM1-TM4) and the downstream C-terminal parts of the native VANGL1 protein. (B) PCR genotyping of a litter obtained by crossing two Vangl1+/− animals: the wild-type (WT) embryo genomic DNA produced only a 791 nucleotide fragment (embryo number 4, +/+), the Vangl1 heterozygous embryos produced both the wild-type and the insert (411 nucleotides) bands (embryo number 2, +/−), and the Vangl1gt/gt homozygous embryos lack the wild-type and produced only the insert band (embryos number 1 and 3, −/−). (C–F) E17.5 Vangl1+/gt, Vangl2+/Lp double heterozygous animals have craniorachischisis. They are shorter than Vangl1+/gt heterozygous embryos or the wild-type littermates (C) and have closed eyelids (C, D). (C–F) Only double heterozygotes are stained with X-Gal, showing the distribution of VangL1 protein, and they have severe craniorachischisis.
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Cochleas isolated from Vangl1+/gt, Vangl2+/Lp trans-heterozygotes with severe craniorachischisis do not have significant PCP defects. Cochleas isolated from the Vangl1/Vangl2 double heterozygous embryos had 2.5 turns, just like the cochleas from the wild-type littermates (A). (B–E) Cell organization in the basal and apical regions of cochlea was similar in the mutants and in the wild-type animals. Therefore, the convergent extension phenotype that is characteristic of other PCP mutants including the Vangl2−/− animals was not detected in our Vangl1/Vangl2 double heterozygotes with craniorachischisis. (B, D) Only minor polarity defects (misalignment of cells) were observed in the Vangl1/Vangl2 double heterozygous mutants. 6 mutant cochleas were analyzed.
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Vangl1gt/gt adults that are viable and fertile produce both VL1-βGeo and VL1-WT mRNAs as well as the VL1-WT protein. The low penetrance of the Vangl1−/− embryonic lethal phenotype prompted us to examine expression of the Vangl1-βGeo fusion and Vangl1 WT mRNAs in Vangl1gt/gt adult tissues. To do so, we prepared mRNA and protein samples from cerebellum and found that VL1 protein is abundantly expressed in this adult tissue (not shown). (A) Position of primers that were used for RT-PCR is marked (>, <). To detect the Vangl1-βGeo fusion mRNA, we used oligo-dT to obtain cDNA for subsequent PCR reaction with Ex3F and BGeo-R1 primers that produced a ~480 nucleotide RT-PCR product. To detect Vangl1 WT mRNA, we used oligo-dT to obtain cDNA for subsequent PCR reaction with 117-For and 996-Rev primers. The ~880 nucleotide PCR product would be obtained only if βGeo was spliced out and Vangl1-WT mRNA was produced. (B) Prior to RT-PCR, animals were re-genotyped and comparison was carried out between the wild-type (CD1) mouse, three Vangl1+/gt heterozygotes and three Vangl1gt/gt homozygotes. (C) RT-PCR for Vangl1-βGeo and Vangl1 WT mRNAs: CD1 animals made only Vangl1 WT mRNA. All other animals made varying amounts of Vangl1-βGeo and Vangl1 WT mRNAs. Similarly, they made different amounts of the VANGL1-WT protein which migrated as approximately 60 kD band when isolated from cerebellum (D, D'). (E, E') Expression of LacZ was analyzed in Vangl1+/gt embryos. Example from two litters is shown (E, E'). (E') A litter containing two Vangl1gt/gt embryos: the first embryo on the left is normal and the third embryo from the left has a turning phenotype. This example demonstrates that one Vangl1gt/gt animal was phenotypically “rescued” (first embryo from the left) and the other one was not, presumably by varying alternative splicing of the mutant transcript to produce varying levels of VANGL1 wild-type protein. Further, two Vangl1+/gt embryos from the same litter (E'), produced varying amounts of VANGL1-βGeo fusion protein. Staining of all embryos was performed at the same time and under identical conditions.
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Vangl2 RNA is expressed in the GRP. (A, B) Shown are dissected GRPs from stage 16/17 embryos that were probed with digoxigenin labeled antisense probes against a-tubulin (A–A″) or Vangl2 RNA (b–b″). Dorsal views are shown in A and B, with ventral views showing expression in the GRP in A' and B'. After imaging, the dissected GRPs were cut in half and imaged from in cross-section. The ventral, or GRP side, is up in panels A″ and B″ and expression in the GRP is marked by arrows.
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Newly generated antibody to VANGL1 protein is highly specific. Specificity of the VANGL1 antibody was tested by Western blotting (A, B). (A) Antibody to VANGL1 detects only the VANGL1 or the YFP-VANGL1 protein and not the VANGL2 or the YFP-VANGL2 protein in extracts of transfected HeLa cells. HeLa cells were transfected with vectors expressing VANGL1 (VL1), VANGL2 (VL2), as well as the corresponding YFP fusion proteins (YFP-VL1 and YFP-VL2). Lysates containing over-expressed proteins were analyzed by Western blots and compared to lysates of untransfected HeLa cells (–) or to vector-transfected cells (vector). Western blots were probed with the affinity-purified antibody to VL1 protein or with the antibody to GFP protein. Blots were also probed for tubulin as a loading control. (B) Antibody to VANGL1 detects a single band in extracts made from P3 vestibular sensory epithelia. The protein detected by the VANGL1 antibody has a higher molecular mass (~100-kD) than the predicted ~60-kD. Protein of the predicted size is detected after endoglycosidaseF treatment of lysates, demonstrating that glycosylation is the main reason for the observed discrepancy in size. The band observed in HeLa cell lysates transfected with VL1 is ~60-kD.
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We thank Ljiljana Milenkovic for numerous discussions, comments on the manuscript and technical guidance throughout the course of this work; Eszter Vladar and Alison McGuigan for discussions and comments on the manuscript: Klara Fekete for help with genotyping; Jeremy F. Reiter for technical advice on mounting of the node-stage embryos; and members of the Axelrod and Scott laboratories for continuous encouragement. We are very thankful to Hiroshi Hamada for providing Pitx2 cDNA.
Conceived and designed the experiments: DA JLS CK MPS JDA. Performed the experiments: DA JLS KS. Analyzed the data: DA JLS CK MPS JDA. Wrote the paper: DA JLS CK MPS JDA.
- 1. Basu B, Brueckner M (2008) Cilia multifunctional organelles at the center of vertebrate left-right asymmetry. Curr Top Dev Biol 85: 151–174.
- 2. Shiratori H, Hamada H (2006) The left-right axis in the mouse: from origin to morphology. Development 133: 2095–2104.
- 3. Nonaka S, Yoshiba S, Watanabe D, Ikeuchi S, Goto T, et al. (2005) De novo formation of left-right asymmetry by posterior tilt of nodal cilia. PLoS Biol 3: e268.
- 4. Hirokawa N, Tanaka Y, Okada Y, Takeda S (2006) Nodal flow and the generation of left-right asymmetry. Cell 125: 33–45.
- 5. Tabin CJ (2006) The key to left-right asymmetry. Cell 127: 27–32.
- 6. Yoshioka H, Meno C, Koshiba K, Sugihara M, Itoh H, et al. (1998) Pitx2, a bicoid-type homeobox gene, is involved in a lefty-signaling pathway in determination of left-right asymmetry. Cell 94: 299–305.
- 7. Campione M, Ros MA, Icardo JM, Piedra E, Christoffels VM, et al. (2001) Pitx2 expression defines a left cardiac lineage of cells: evidence for atrial and ventricular molecular isomerism in the iv/iv mice. Dev Biol 231: 252–264.
- 8. Schweickert A, Weber T, Beyer T, Vick P, Bogusch S, et al. (2007) Cilia-driven leftward flow determines laterality in Xenopus. Curr Biol 17: 60–66.
- 9. Vick P, Schweickert A, Weber T, Eberhardt M, Mencl S, et al. (2009) Flow on the right side of the gastrocoel roof plate is dispensable for symmetry breakage in the frog Xenopus laevis. Dev Biol 331: 281–291.
- 10. Blum M, Beyer T, Weber T, Vick P, Andre P, et al. (2009) Xenopus, an ideal model system to study vertebrate left-right asymmetry. Dev Dyn 238: 1215–1225.
- 11. Wang Y, Nathans J (2007) Tissue/planar cell polarity in vertebrates: new insights and new questions. Development 134: 647–658.
- 12. Etheridge SL, Ray S, Li S, Hamblet NS, Lijam N, et al. (2008) Murine dishevelled 3 functions in redundant pathways with dishevelled 1 and 2 in normal cardiac outflow tract, cochlea, and neural tube development. PLoS Genet 4: e1000259.
- 13. Saburi S, Hester I, Fischer E, Pontoglio M, Eremina V, et al. (2008) Loss of Fat4 disrupts PCP signaling and oriented cell division and leads to cystic kidney disease. Nat Genet 40: 1010–1015.
- 14. Axelrod JD (2009) Progress and challenges in understanding planar cell polarity signaling. Semin Cell Dev Biol 20(8): 964–71.
- 15. Strutt H, Strutt D (2009) Asymmetric localisation of planar polarity proteins: Mechanisms and consequences. Semin Cell Dev Biol 20(8): 957–63.
- 16. Klein TJ, Mlodzik M (2005) Planar cell polarization: an emerging model points in the right direction. Annu Rev Cell Dev Biol 21: 155–176.
- 17. Wang J, Hamblet NS, Mark S, Dickinson ME, Brinkman BC, et al. (2006) Dishevelled genes mediate a conserved mammalian PCP pathway to regulate convergent extension during neurulation. Development 133: 1767–1778.
- 18. Wang Y, Guo N, Nathans J (2006) The role of Frizzled3 and Frizzled6 in neural tube closure and in the planar polarity of inner-ear sensory hair cells. J Neurosci 26: 2147–2156.
- 19. Montcouquiol M, Rachel RA, Lanford PJ, Copeland NG, Jenkins NA, et al. (2003) Identification of Vangl2 and Scrb1 as planar polarity genes in mammals. Nature 423: 173–177.
- 20. Montcouquiol M, Sans N, Huss D, Kach J, Dickman JD, et al. (2006) Asymmetric localization of Vangl2 and Fz3 indicate novel mechanisms for planar cell polarity in mammals. J Neurosci 26: 5265–5275.
- 21. Deans MR, Antic D, Suyama K, Scott MP, Axelrod JD, et al. (2007) Asymmetric distribution of prickle-like 2 reveals an early underlying polarization of vestibular sensory epithelia in the inner ear. J Neurosci 27: 3139–3147.
- 22. Hamblet NS, Lijam N, Ruiz-Lozano P, Wang J, Yang Y, et al. (2002) Dishevelled 2 is essential for cardiac outflow tract development, somite segmentation and neural tube closure. Development 129: 5827–5838.
- 23. Seifert JR, Mlodzik M (2007) Frizzled/PCP signalling: a conserved mechanism regulating cell polarity and directed motility. Nat Rev Genet 8: 126–138.
- 24. Winter CG, Wang B, Ballew A, Royou A, Karess R, et al. (2001) Drosophila Rho-associated kinase (Drok) links Frizzled-mediated planar cell polarity signaling to the actin cytoskeleton. Cell 105: 81–91.
- 25. Crompton LA, Du Roure C, Rodriguez TA (2007) Early embryonic expression patterns of the mouse Flamingo and Prickle orthologues. Dev Dyn 236: 3137–3143.
- 26. Torban E, Patenaude AM, Leclerc S, Rakowiecki S, Gauthier S, et al. (2008) Genetic interaction between members of the Vangl family causes neural tube defects in mice. Proc Natl Acad Sci U S A 105: 3449–3454.
- 27. Veeman MT, Axelrod JD, Moon RT (2003) A second canon. Functions and mechanisms of beta-catenin-independent Wnt signaling. Dev Cell 5: 367–377.
- 28. Kaufman MH (1992) The atlas of mouse development. London; San Diego: Academic Press.
- 29. Mitchell B, Stubbs JL, Huisman F, Taborek P, Yu C, et al. (2009) The PCP pathway instructs the planar orientation of ciliated cells in the Xenopus larval skin. Curr Biol 19: 924–929.
- 30. Marshall WF, Kintner C (2008) Cilia orientation and the fluid mechanics of development. Curr Opin Cell Biol 20: 48–52.
- 31. Hashimoto M, Shinohara K, Wang J, Ikeuchi S, Satoko Y, et al. Planar polarization of node cells determines the rotational axis of the node cilia. Nat Cell Biol. in press.
- 32. Park TJ, Mitchell BJ, Abitua PB, Kintner C, Wallingford JB (2008) Dishevelled controls apical docking and planar polarization of basal bodies in ciliated epithelial cells. Nat Genet 40: 871–879.
- 33. Jiang D, Munro EM, Smith WC (2005) Ascidian prickle regulates both mediolateral and anterior-posterior cell polarity of notochord cells. Curr Biol 15: 79–85.
- 34. Ciruna B, Jenny A, Lee D, Mlodzik M, Schier AF (2006) Planar cell polarity signalling couples cell division and morphogenesis during neurulation. Nature 439: 220–224.
- 35. Yin C, Kiskowski M, Pouille PA, Farge E, Solnica-Krezel L (2008) Cooperation of polarized cell intercalations drives convergence and extension of presomitic mesoderm during zebrafish gastrulation. J Cell Biol 180: 221–232.
- 36. Sive H GR, Harland RM (1998) The early development of Xenopus laevis: a laboratory manual. Plainview, NY: Cold Spring Harbor Press.
- 37. Stubbs JL, Oishi I, Izpisua Belmonte JC, Kintner C (2008) The forkhead protein Foxj1 specifies node-like cilia in Xenopus and zebrafish embryos. Nat Genet 40: 1454–1460.
- 38. Stubbs JL, Davidson L, Keller R, Kintner C (2006) Radial intercalation of ciliated cells during Xenopus skin development. Development 133: 2507–2515.
- 39. Nasevicius A, Ekker SC (2000) Effective targeted gene ‘knockdown’ in zebrafish. Nat Genet 26: 216–220.
- 40. Heasman J (2002) Morpholino oligos: making sense of antisense? Dev Biol 243: 209–214.
- 41. Harland RM (1991) In situ hybridization: an improved whole-mount method for Xenopus embryos. Methods Cell Biol 36: 685–695.