PCP and Wnt pathway components act in parallel during zebrafish mechanosensory hair cell orientation

Article metrics


Planar cell polarity (PCP) plays crucial roles in developmental processes such as gastrulation, neural tube closure and hearing. Wnt pathway mutants are often classified as PCP mutants due to similarities between their phenotypes. Here, we show that in the zebrafish lateral line, disruptions of the PCP and Wnt pathways have differential effects on hair cell orientations. While mutations in the PCP genes vangl2 and scrib cause random orientations of hair cells, mutations in wnt11f1, gpc4 and fzd7a/b induce hair cells to adopt a concentric pattern. This concentric pattern is not caused by defects in PCP but is due to misaligned support cells. The molecular basis of the support cell defect is unknown but we demonstrate that the PCP and Wnt pathways work in parallel to establish proper hair cell orientation. Consequently, hair cell orientation defects are not solely explained by defects in PCP signaling, and some hair cell phenotypes warrant re-evaluation.


Cell polarity is crucial for the function of many tissues and its establishment during development has fascinated many generations of biologists. In addition to the well-studied apico-basal polarity of cells, cells are also coordinately aligned in the plane of a tissue’s axis, termed planar cell polarity (PCP). PCP relies on the asymmetric distribution of core PCP components, such as Van Gogh/Vangl, Frizzled, Disheveled, Prickle/Spiny-Legs, and Fmi/Celsr and Diego1,2,3,4. This pathway was discovered in insects5,6,7,8 and subsequently also identified in vertebrates9,10,11. PCP is required during key developmental processes that shape the embryo, such as gastrulation and neural tube closure1,2,3, however, how PCP is initiated is poorly understood. One proposed mechanism is that Wnt gradients act as instructive morphogens that initiate the molecular asymmetry of PCP components12,13,14,15,16,17. However, in some contexts Wnt ligands are required but not instructive (permissive) to drive PCP-dependent processes18,19,20. In this study, we set out to investigate the role of Wnt signaling in polarizing sensory hair cells.

The vertebrate inner ear is a classical model to study the function of the PCP pathway, as stereocilia bundle coordination is very sensitive to changes in PCP21,22. Wnt gradients have been implicated in establishing PCP in the ear23,24 but due to the inaccessibility of the ear, the study of the function of the PCP and Wnt signaling pathways in coordinating hair cell alignment is challenging to investigate.

A more experimentally accessible model to study hair cell orientation is the sensory lateral line system of aquatic vertebrates that detects water movements across the body of the animal25,26. Because of its superficial location in the skin, the lateral line is amenable to experimental manipulations and live imaging27. The lateral line system consists of volcano-shaped sensory organs (neuromasts) that are composed of mantle cells on the outside and support cells and mechanosensory hair cells in the center (Fig. 1a, b 25). The mechanosensory hair cells are homologous to the ones found in the inner ear28,29. The sensory organs are derived from several neurogenic, cephalic placodes/primordia that either migrate into the trunk or into the head30. As they migrate, primordia periodically deposit clusters of cells that differentiate into sensory organs31,32,33. PrimordiumI (primI) and primordiumII (primII) both migrate into the trunk but arise from different placodes (primary placode and D0 placode, respectively). The D0 placode also gives rise to a third primordium that migrates onto the dorsal side of the trunk, called primD25,34.

Fig. 1

Mutations in the Wnt and PCP pathways affect the hair cell alignment in the lateral line. a Confocal image of a 5 days post fertilization (dpf) Tg(cldnb: lynGFP); Tg(sqet4); Tg(cldnb:H2A-mCherry) larva. b Schematic lateral view of a 5 dpf neuromast showing the different cell types. c Diagram of a 5 dpf larva showing the two different orientations of primI and primII-derived hair cells. d In situ hybridization of wnt11 (wnt11f1) in primI and primII-derived 5 dpf neuromasts. ej Phalloidin stainings show hair cell orientations in primI-derived neuromasts of wild type (e), Wnt pathway mutants (fh) and PCP mutants (ij; Fisher’s Exact Test p-val for vangl2 primI = 7.33 × 10−28, MZscrib primI = 1.41 × 10−17). Individual hair cell orientation is depicted for each of the conditions tested. Black arrows denote disruption of the wild-type orientation. The Rose diagrams show the hair cell orientation distribution with respect to the longitudinal axis of the animal (horizontal) (WT n = 194 hair cells, MZwnt11 (wnt11f1) n = 353, gpc4 n = 222, MZfzd7a/7b n = 74, vangl2 n = 226, MZscrib n = 535). Bottom right depicts the Fisher’s exact test comparison with respect to the wild type for each condition. Top right shows the binomial test for each condition. kp Phalloidin staining shows hair cell orientation in primII-derived neuromasts of wild type (k), Wnt pathway mutants (ln Fisher’s Exact Test p-val for MZwnt11 (wnt11f1) primII = 1.69 × 10−23, gpc4 primII = 6.93 × 10−31, MZfzd7a/7b primII = 3.91 × 10−33) and PCP mutants (op, vangl2 primII p = 2.52 × 10−21, MZscrib primII = 9.22 × 10−12). Individual hair cell orientation is depicted for for each of the conditions tested and the color code is the same as in (ej). The Rose diagrams reflect the same as in (ej) (WT n = 209 hair cells, MZwnt11 (wnt11f1) n = 295, gpc4 n = 214, MZfzd7a/7b n = 182, vangl2 n = 141, MZscrib n = 392). For ep, comparisons of angle distributions with respect to wild type, Fisher’s Exact Test ***p < 0.001, N.S not significant, binomial test A-P ***p < 0.001, A-P* = p < 0.05. e”–p”. A-P anteroposterior orientation, D-V dorsoventral orientation. Scale bar in a equals 500 μm, d equals 20 μm, e equals 5 μm

Hair cells possess short actin-rich stereocilia adjacent to a tubulin-rich, long kinocilium. Each hair cell is planar polarized with the long microtubule-based kinocilium localized to one pole of the cuticular plate (Fig. 1b). Within a sensory organ, hair cells arise in pairs with their kinocilia pointing toward each other but are aligned along a common axis (Fig. 1c). The positioning of the kinocilium along this axis is controlled by Notch signaling/Emx2 and its loss causes all hair cells within a neuromast to point into the same direction35,36. PrimI and primII-derived hair cells show different axial polarities, allowing the animal to sense water flow from different directions (Fig. 1c 37). In primI-derived trunk neuromasts, hair cells are planar polarized along the anterioposterior (A-P) axis and hair cells in primII-derived neuromasts are aligned along the dorsoventral (D-V) axis. The differential hair cell orientation has been correlated with the different directions of primI and primII migration, however, no underlying mechanism has been identified25,34,37. At the single hair cell level, previous reports have suggested that PCP regulates hair cell progenitor orientation by controlling cell division angles and cell rearrangements38,39. Yet the molecular code for how different neuromast axial orientations and individual hair cell orientations are coordinated remains ill understood.

Here, we show that loss of PCP and Wnt pathway genes (wnt11 (wnt11f1) (formerly known as wnt11r, wnt11-related40), gpc4 and fzd7a/7b) have different consequences on hair cell orientations. While mutations in the PCP genes vangl2 and scrib cause disorganized hair cell orientations in all neuromasts, mutations in the Wnt pathway genes wnt11 (wnt11f1), gpc4 and fzd7a/7b show a striking concentric pattern of hair cell orientation in only primII neuromasts. As neither the core PCP component Vangl2, nor Notch/Emx2 signaling are affected in Wnt pathway mutants we conclude that the Wnt pathway acts in parallel to these pathways. In addition, the concentric hair cell phenotype in Wnt pathway mutants is caused by the disruption of coordinated organization of the surrounding support cells, rather than by affecting the axis of polarity or kinocilium positioning in individual hair cells.

The expression patterns of Wnt pathway genes suggest that the Wnt pathway acts very early in lateral line development. Thus, Wnt signaling does not instruct PCP, but acts to coordinate support cell organization during the formation and migration of the primordium before the appearance of hair cells. The molecular mechanisms by which Wnt signaling coordinates support cell orientation remains to be elucidated. Overall, our findings demonstrate that hair cell orientation defects cannot solely be attributed to defects in the PCP pathway and that some phenotypes formerly characterized as PCP defects need to be re-evaluated.


Wnt and PCP genes cause different hair cell orientation phenotypes

During a large in situ screen, we unexpectedly observed asymmetric expression of wnt11 (wnt11f1), the ortholog of mammalian WNT1140. wnt11 (wnt11f1) is expressed along the anterior edge of only primI-derived neuromasts, but is absent from primII-derived neuromasts (Fig. 1d, Supplementary Fig. 1). Since Wnt ligands can instruct planar polarization of cells10,16,17,41,42,43,44, we hypothesized that wnt11 (wnt11f1) establishes hair cell orientation by directing PCP in primI-derived neuromasts. We measured hair cell orientation in the cuticular plate using Phalloidin, which labels actin-rich stereocilia but not the tubulin-rich kinocilium (Fig. 1b). We used the kinocilium position to determine the axis of polarity of each hair cell. Phalloidin stainings of sibling primI-derived neuromasts show that hair cells possess a significant orientation bias parallel to the A-P axis based on the angles with respect to the horizontal in rose diagrams (Fig. 1e). In contrast, primII-derived neuromasts show an orientation bias along the D-V axis (Fig. 1k). Furthermore, neighboring hair cells in both primordia show coordinated polarities (Supplementary Fig. 1c, i). Unexpectedly, zygotic and maternal zygotic (MZ) mutations in wnt11 (wnt11f1) do not affect hair cell orientation in primI-derived neuromasts in which wnt11 (wnt11f1) is expressed (Fig. 1f; Supplementary Fig. 1d), but disrupt the hair cell orientation in primII-derived neuromasts (Fig. 1l; Supplementary Fig. 1j). Even though zygotic wnt11 (wnt11f1) mutants also show the phenotype, we from here on used MZwnt11 (wnt11f1) larvae to increase the number of mutant fish for our studies.

gpc4 (glypican4, a heparan sulfate proteoglycan (HSPG)) and fzd7 (a frizzled-class receptor) interact with Wnt ligands during convergent extension (CE), and we tested whether mutations in these genes also cause hair cell polarity defects18,45,46,47,48,49,50,51. Indeed, gpc4 and MZfzd7a/7b mutants show the same concentric hair cell phenotype as MZwnt11 (wnt11f1) mutants suggesting they act in the same pathway (Fig. 1g, m; and h, n; Supplementary Fig. 1e, f, k, l). This interpretation is supported by the finding that wnt11 (wnt11f1);gpc4 double mutants possess the same phenotype as the single mutants (Supplementary Fig. 1o). gpc4 and fzd7a/7b also interact with wnt11f2 (formerly called wnt11/silberblick,40) during CE18,50,51. We, therefore, wondered if wnt11f2 mutants also possess hair cell defects and if wnt11f2 possibly interacts with wnt11 (wnt11f1). However, wnt11f2 mutants have normal hair cell orientations, as do wnt11 (wnt11f1);wnt11f2 double heterozygous animals, indicating that these two paralogs do not interact (Supplementary Fig. 1p).

Since gpc4 and MZfzd7a/7b mutants have been described as PCP signaling mutants in other contexts45,46,52,53, we compared the phenotypes of MZwnt11 (wnt11f1), gpc4 and MZfz7a/7b mutants to the hair cell phenotype of the PCP mutants vangl2 and scribble (scrib). A mutation in the core PCP gene vangl2 disrupts hair cell orientation in both primI and primII-derived neuromasts38,39 (Fig. 1i, o; Supplementary Fig. 1g, m). Scribble1 interacts with the PCP pathway in the mouse cochlea and its loss causes hair cell defects54,55. Likewise, we observed that MZscrib zebrafish mutants show a significant deviation of hair cell orientations in both primI and primII-derived neuromasts (Fig. 1j, p). However, the phenotype is not as severe as in vangl2 mutants and primI and primII neuromasts still show a bimodal distribution along the A-P and D-V axes, respectively (Fig. 1j, p; Supplementary Fig. 1h, n). Therefore, scrib likely acts partially redundantly with other PCP proteins. These results suggest that while PCP genes are required to establish proper hair cell orientation in all neuromasts, wnt11 (wnt11f1), gpc4 and fzd7a/7b (from now on referred to as Wnt pathway genes), affect hair cell orientation only in primII-derived neuromasts.

Mutations in both Wnt and PCP pathway genes result in misorientation of hair cells. However, we found that mutations in Wnt pathway genes cause hair cells in primII-derived neuromasts to orient in a striking concentric fashion (Fig. 2b, g; Supplementary Fig. 2b–f), whereas in vangl2 mutants hair cells are oriented randomly (Fig. 2c, h; Supplementary Fig. 1g, m). Likewise, hair cells in the other PCP signaling mutant MZscrib do not arrange in a concentric fashion (Supplementary Fig. 2d, g). This difference in phenotype suggests that the Wnt and PCP signaling pathways control hair cell orientation in parallel, rather than through a common pathway. However, Wnt and PCP pathways have been described to interact genetically in the establishment of hair cell orientation in the inner ear24. To assess a possible genetic interaction between vangl2 and wnt11 (wnt11f1) in lateral line neuromasts we generated double homozygous vangl2 and MZwnt11 (wnt11f1) larvae. In double homozygous fish, primI-and II-derived neuromasts show random hair cell orientation (Fig. 2e, j; Supplementary Fig. 2h, i). In addition, the concentric phenotype shown by primII neuromasts of MZwnt11 (wnt11f1) single mutants (Fig. 2i; Supplementary Fig. 2j) disappears in the double MZwnt11 (wnt11f1);vangl2 mutants (Fig. 2j; Supplementary Fig. 2k). Due to the genetic compensation between Vangl2 and Vangl1 in the mammalian inner ear56,57, we tested if vangl1 and vangl2 act redundantly during zebrafish lateral line hair cell orientation. Indeed, vangl1 is expressed in the migrating primI and a few mantle cells in 32 and 50 h post fertilization (hpf) neuromasts (Supplementary Fig. 2l). A t-SNE plot of 5 dpf embryos also shows that a few mantle cells are positive (Supplementary Fig. 2m). However, vangl1 is not expressed in the migrating primII (Supplementary Fig. 2l). We generated vangl1 CRISPants which are characterized by shortened, curly tails and notochord defects reminiscent of PCP mutants (Supplementary Fig. 2o 11,45,58,59). However, these embryos do not show a disruption in their hair cell orientation (Supplementary Fig. 2p). In addition, neither MZwnt11 (wnt11f1) or vangl2 mutants injected with vangl1 CRISPR show a deviation from the phenotypes observed in uninjected MZwnt11 (wnt11f1) or vangl2 mutants (Supplementary Fig. 2q, r; Fig. 2b, c, g, h). These findings suggest that vangl1 and vangl2 do not act redundantly during the establishment of hair cell orientation in the lateral line. In sum, the disorganized hair cell phenotype caused by a mutation in vangl2 is epistatic over the concentric phenotype observed in wnt11 (wnt11f1) embryos, providing additional support for the hypothesis that the PCP and Wnt pathways work in parallel and have different roles during the establishment of hair cell orientation in primII-derived neuromasts.

Fig. 2

PCP and Wnt pathway mutants possess different hair cell phenotypes. In PCP mutants hair cells are randomly oriented, whereas hair cells in primII of Wnt pathway mutants show a concentric orientation pattern. ae Phalloidin images show the cell polarity axis (yellow lines) in primI-derived neuromasts of wild type (a), Wnt pathway mutant MZwnt11 (wnt11f1) (b), PCP mutant vangl2 (c), single MZwnt11 (wnt11f1) siblings (d), and double MZwnt11 (wnt11f1);vangl2 larvae (e) homozygous mutant hair cells and their distribution of angles with respect to the nearest ellipse tangent (concentricity). Note that none of the conditions shows significant concentricity (uniform distribution p-values in a = 0.423, b = 0.054, c = 0.464, d = 0.165, e = 0.077, f = 0.019; WT n = 194 hair cells, MZwnt11 (wnt11f1) n = 353, vangl2 n = 226, MZwnt11 (wnt11f1);vangl2 sibling n = 276, MZwnt11 (wnt11f1);vangl2 doubles n = 406). The Von Mises distributions are shown in red for visual display of the data distribution. fj Phalloidin images show the cell polarity axis (yellow lines) in primII-derived neuromasts of wild type (f), Wnt pathway mutant wnt11 (wnt11f1) (g), PCP mutant vangl2 (h), single MZwnt11 (wnt11f1) siblings (i) and double MZwnt11 (wnt11f1);vangl2 (j) homozygous mutants and their distribution of angles with respect to the nearest ellipse tangent (concentricity). Note that only the Wnt pathway mutants (g, i) show significant concentricity (Uniform distribution p-values in f = 0.314, g = 1.28 × 10−27, h = 0.86, i = 02.92 × 10−19, j = 0.298; WT n = 209 hair cells, MZwnt11 (wnt11f1) n = 295, vangl2 n = 141, MZwnt11 (wnt11f1);vangl2 sibling n = 252, MZwnt11 (wnt11f1);vangl2 doubles n = 365). The von Mises distributions are shown in red for visual display of the data distribution. Yellow lines in aj indicate the hair cell polarity axis, determined by the position of the kinocilium. Not Concentric vs Concentric labels were based on calculations in (aj). Scale bar equals 5 μm

Vangl2 localization is not affected in Wnt pathway mutant hair cells

Since loss of vangl2 disrupts the concentric phenotype, we hypothesized that PCP signaling might be correctly established in hair cells of the Wnt pathway mutants. To test whether one of the landmarks of PCP signaling, asymmetric distribution of Vangl23, is disrupted in hair cells of Wnt pathway mutants we performed anti-Vangl2 antibody stainings in 5 dpf neuromasts (Fig. 3). In wild type neuromasts, Vangl2 is asymmetrically enriched in approximately 90% of hair cells. Vangl2 is localized to the posterior side of hair cells in primI-derived neuromasts (Fig. 3a) and to the ventral side of hair cells in primII-derived neuromasts (Fig. 3e, i). However, as hair cells in a wild type neuromast possess two different orientations (Fig. 1b, c) only approximately half of the hair cells show Vangl2 signal in the same pole as the kinocilium (Supplementary Fig. 3a), which agrees with previous reports using a fluorescent reporter or a Vangl2 antibody36,39.

Fig. 3

Vangl2 asymmetry is not affected in hair cells of MZwnt11 (wnt11f1) mutants. ad Double β-II-Spectrin (labeling the cuticular plates) and Vangl2 immunodetection in primI neuromasts of 5 dpf wild type (a), MZscrib mutants (b), scrib siblings (c) and MZwnt11 (wnt11f1) mutants (d). eh Double β-II-Spectrin (labeling the cuticular plates) and Vangl2 immunodetection in primII neuromasts of 5 dpf wild type (e), MZscrib mutants (f), scrib siblings (g) and MZwnt11 (wnt11f1) mutants (h). i Quantification of the percentage of hair cells that show asymmetric Vangl2 for each of the conditions in both primordia-derived neuromasts. jn Clonal localization of GFP-XVangl2 in hair cells of neuromasts that show primI and primII polarity in wild type (j, k) and MZwnt11 (wnt11f1) mutants (m, n) neuromasts. The majority of the clones were localized in neuromasts in the head, which show the same hair cell orientation as in primI and primII-derived neuromasts in each of the cases. l, o Quantification of GFP-XVangl2 fluorescence around the cuticular plates (360°) of hair cells in neuromasts that show primI and primII polarity of wild type (l) and MZwnt11f mutants (o). p GFP fluorescence and Phalloidin enrichment (polarity ratio, calculated from the cap of max value to the lowest value) in the different conditions analyzed in (l, o). Error bars in l, o, and p represent S.E.M. ***Fisher’s exact test p < 0.01. Scale bar in a equals 5 μm, j equals 2 μm

While Vangl2 staining is not detected in vangl2 mutants (Supplementary Fig. 3b–e), MZscrib mutant fish show reduced signal and only 26.3% of hair cells with asymmetric Vangl2 in primI and primII-derived neuromasts (Fig. 3b, f, i) compared with their siblings (Fig. 3c, g, i). The reduction in signal, rather than the complete loss, agrees with reports in the mouse cochlea55 and might explain why hair cell disorganization in MZscrib mutants is not as dramatic as in vangl2 mutants. In addition, among the 26.3% of hair cells that that show asymmetric Vangl2 in MZscrib mutants, approximately 10% of hair cells show randomized Vangl2 localization that is not correlated with the position of the kinocilium (Supplementary Fig. 3a). Together with the finding that only 26.3% of MZscrib hair cells show asymmetric distribution of Vangl2, this indicates that PCP signaling is affected in MZscrib. In contrast to the PCP mutants, MZwnt11 (wnt11f1) mutants possess asymmetric distribution of Vangl2 in hair cells of both primI and primII-derived neuromasts showing that PCP signaling is not affected (Fig. 3d, h, i; Supplementary Fig. 3a). To further test whether hair cells in MZwnt11 (wnt11f1) mutants show asymmetric Vangl2 localization, we generated a hair cell-specific promoter-driven GFP-Vangl2 Tg(myo6b:GFP-XVangl2). We then calculated GFP fluorescence enrichment around the circumference (−180° to 180°) of the cuticular plate at the base of the stereo- and kinocilia with 0° on the x-axis being the point of maximum intensity (Fig. 3j–o). In wild-type larvae mosaic expression of fluorescent Vangl2 is asymmetrically enriched in hair cells of primI and primII-derived neuromasts (Fig. 3j–l, p). In MZwnt11 (wnt11f1) mutants, GFP-Vangl2 is asymmetrically localized in primI and primII-derived neuromasts like in wild type hair cells (Fig. 3m–p). These results indicate that in contrast to the PCP mutant vangl2, individual hair cell PCP is normal in Wnt pathway mutants. These findings suggest that the concentric arrangement of hair cells in Wnt pathway mutants is caused by a PCP-independent mechanism.

The Wnt and PCP pathways have different temporal requirements

The differences in the hair cell orientation phenotypes of Wnt and PCP pathway mutants suggest that they do not act in the same pathway. To identify further differences in their phenotypes we investigated PCP-dependent cell behaviors of hair cell progenitors in vivo. The two daughters of a hair cell progenitor often change their position with respect to each other before differentiating38,39 (Supplementary Movie 1). These cell rearrangements and their duration depend on functional PCP signaling during development and regeneration. In vangl2 mutants the hair cell rearrangements do not lead to complete reversal of positions, they sometimes occur multiple times and their duration is prolonged39. In contrast, time-lapse analyses of the behavior of developing hair cell progenitors in primII-derived neuromasts of MZwnt11 (wnt11f1) mutants reveals no significant differences in the number of times they rearrange, the duration of the rearrangements or the angle of divisions with respect to the radius of the neuromast compared to wild type (Supplementary Fig. 4a–f). We conclude that hair cell pairs arise normally in MZwnt11 (wnt11f1) mutants. We also identified differences in the timing of the onset of the hair cell phenotypes between PCP and Wnt pathway mutants. In wild type larvae a pair of hair cells develops from a common progenitor38 with the kinocilia of both hair cells pointing towards each other in 96% of the cases (Fig. 4a). The first pair of hair cells in MZwnt11 (wnt11f1) mutants shows correct orientation 69% of the time (Fig. 4b), while in vangl2 mutants they orient properly only in 23% of the cases (Fig. 4c). We conclude that the majority of MZwnt11 (wnt11f1) mutant hair cells possess the proper orientation with respect to their sister hair cell as they form, whereas most vangl2 mutant hair cells show defective hair cell polarities that are not coordinated with their sister hair cell as soon as the hair cell progenitor divides.

Fig. 4

Differences in the appearance of the hair cell phenotypes in vangl2 and MZwnt11 (wnt11f1) mutants. ac Orientation of the first pair of hair cells in primII-derived neuromasts of wild type (a), MZwnt11 (wnt11f1) mutants (b), and vangl2 mutants (c) labeled with Tg(myo6b:β-Actin-GFP). In c, the left panel shows the number of correctly oriented pairs, and the right panel shows the number of incorrectly oriented pairs (the majority). The percentages for each of the conditions represent the number of pairs that show correct hair cell orientation. df Hair cell orientation over time in wild type (n = 3 animals) (d), MZwnt11 (wnt11f1) mutants (n = 5) (e), and vangl2 mutants (n = 2) (f) labeled with Tg(myo6b:β-Actin-GFP). Each of the conditions is depicted using a color-coded cartoon, and the hair cell orientation of the first pair is represented by arrows in the box on the lower right. To differentiate between each hair cell of the pair, each of the arrows is in a different color. gj Hair cell orientation of the same vangl2 mutant fish at 4 dpf (g) and 5 dpf (h), and the same MZwnt11 (wnt11f1) mutant embryo at 4 dpf (i) and 5 dpf (j) in a Tg(myo6b:β-Actin-GFP) transgenic background. The distribution of angles of each given hair cell with respect to the nearest ellipse tangent (concentricity) for primII-derived neuromasts of all the conditions tested is shown. Note that only the MZwnt11 (wnt11f1) mutants at 5 dpf (j) show significant concentricity (Uniform distribution p-values in g = 0.223, h = 0.469, i = 0.308, j = 1.97 × 10−07). The von Mises distribution is shown for visual display of the data distribution. Yellow lines represent the polarity axis for each hair cell. “Not Concentric” vs. “Concentric” labels in gj were based on the statistical significance (n = 8 neuromasts for each condition). Scale bars in a, d, and g equal 2 μm

As MZwnt11 (wnt11f1) mutant hair cells eventually all show orientation defects with respect to their sister hair cell, we asked if this phenotype arises progressively. We measured the polarity of the first hair cell pair over time as additional hair cells appear and observed that in wild-type neuromasts the hair cells keep pointing towards each other or their polarity is even refined (Fig. 4d; Supplementary Movie 2). In contrast, in MZwnt11 (wnt11f1) mutants the correct orientation is progressively lost (Fig. 4e; Supplementary Movie 3). In vangl2 mutants, the aberrant polarity of the first pair also changes over time (Fig. 4f; Supplementary Movie 4). At this point, we do not understand if this effect of cell crowding on the Wnt and PCP phenotypes is caused by the same mechanism or not.

As 5 dpf vangl2 hair cells do not arrange in concentric circles, we asked whether concentricity might be an intermediate state that is subsequently lost in PCP mutants. We performed time-lapse analyses of developing hair cells in vangl2 and MZwnt11 (wnt11f1) neuromasts between 4 and 5 dpf. vangl2 hair cells never arrange in a concentric fashion and are always randomly oriented (Fig. 4g, h; Supplementary Fig. 4g). Thus, concentricity is not a property of developing PCP-deficient hair cells at any stage of their development. Likewise, 4 dpf MZwnt11 (wnt11f1) (Fig. 4i) mutant hair cells are not organized in a concentric fashion, even though they are misaligned (Supplementary Fig. 4g). However, starting at 5 dpf, concentricity is detected in MZwnt11 (wnt11f1) mutants (Fig. 4j; Supplementary Fig. 4g). Therefore, concentricity arises over time in MZwnt11 (wnt11f1) mutants as more hair cells are being added. We conclude that the hair cell defects in PCP and Wnt pathway mutants are caused by different mechanisms, because the majority of vangl2 mutant hair cells are already misaligned with respect to their sister hair cell after progenitor division, whereas the misalignment of the two sister hair cells in MZwnt11 (wnt11f1) mutant hair cells arises over time.

Wnt pathway genes coordinate support cell organization

As the hair cell defect arises over time in MZwnt11 (wnt11f1) mutants we wondered if the hair cell phenotype could be secondary to defects in neighboring support cells. Support cells surround and sit underneath developing hair cells and serve as hair cell progenitors38,60,61. Interestingly, support cells are aligned along the A-P and D-V axes in primI and primII-derived neuromasts, respectively, raising the possibility that the Wnt pathway genes might be acting on them (Fig. 5a, b).

Fig. 5

Wnt pathway genes are required for proper coordinated support cell organization. a, b Phalloidin staining of wild-type primI and primII-derived neuromasts. The dotted square outlines the area magnified in (a) and (b). Two support cells each were false colored to depict their orientation. bj Phalloidin staining of neuromasts 3 h after hair cell ablation. c, d Wild-type primI (c) and primII-derived (d) neuromasts. e, f vangl2 mutant primI (e) and primII-derived (f) neuromasts. g, h MZscrib mutant primI (g) and primII-derived (h) neuromasts. i, j MZwnt11 (wnt11f1) mutant primI (i) and primII-derived (j) neuromasts. k, l vangl2;MZwnt11 (wnt11f1) double mutant primI (k) and primII-derived (l) neuromasts. The histograms show the distribution of binned angles of cell orientation with respect to the horizontal for each of the conditions tested. c, d Angle distribution in wild-type primI (c one-way chi square test p = 1.78 × 10−87) and primII-derived (d p = 4.54 × 10−19) neuromasts. Note that primI distribution is skewed toward being horizontally aligned, while the distribution in primII-derived neuromasts is toward vertical alignment. e, f Angle distribution in vangl2 mutant primI (e p = 4.91 × 10−13) and primII-derived (f p = 2.14 × 10−16) neuromasts. g, h Angle distribution in MZscrib mutant primI (g p = 1.40 × 10−14) and primII-derived (h p = 9.60 × 10−13) neuromasts. i, j Support cell orientation in MZwnt11 (wnt11f1) mutant primI (i p = 5.32 × 10−52) and primII-derived (j p = 0.006) neuromasts. k, l Support cell orientation in vangl2;MZwnt11 (wnt11f1) double mutant primI- (k p = 6.69 x 10^-26) and primII-derived (l p = 0.22) neuromasts. m, n Double β-II-Spectrin (labeling the cuticular plates) and ZO-1 staining of a 5 dpf wild-type neuromasts. o, p Wild-type atoh1a CRISPants do not possess hair cells (β-II-spectrin is absent; see also Supplementary Fig. 5) and the support cells in all neuromasts show coordinated orientation (one-way chi-square test p-value in o = 4.98 × 10−20, p = 2.63 × 10−19). q, r MZwnt11 (wnt11f1) injected with atoh1a CRISPR show coordinated support cell orientation in primI-derived neuromasts (q p = 2.88 × 10−60) and do not show coordinated support cell orientation in primII neuromasts (r p = 0.24). Scale bar in a, c, and o equal 5 μm

To better visualize any defects in support cell organization we removed hair cells by soaking the larvae in the antibiotic neomycin62 and calculated their orientation with respect to the horizontal (Supplementary Fig. 5a). In wild-type larvae, support cells show a coordinated, elongated alignment along the horizontal plane (A-P axis) in primI-derived neuromasts (Fig. 5c) and vertical plane (D-V axis) in primII-derived neuromasts (Fig. 5d). These cell alignments demonstrate that hair cell ablation does not disrupt instrinsic support cell alignment. Unexpectedly, we observed that in vangl2 mutants primI-derived support cells are normally aligned along the horizontal axis, even though their hair cell orientation is randomized (Fig. 5e). vangl2 mutant support cells in primII-derived neuromast still align, but offset by 90° horizontally (Fig. 5f), a finding we currently cannot explain. Thus, support cells in primII-derived neuromasts of vangl2 mutants show a cell orientation defect, but not randomization. This suggests the vangl2 might play some not understood role in only primII-derived support cell orientation. However, the MZscrib PCP mutant shows wild type support cell organization in both primI (Fig. 5g) and primII-derived neuromasts (Fig. 5h). These results imply that functional PCP might not be required for coordinated support cell alignment but that PCP genes act mostly in hair cells. On the other hand, in the Wnt pathway mutants MZwnt11 (wnt11f1) and gpc4, primI-derived support cells are horizontally aligned (Fig. 5i), whereas support cells in primII-derived neuromasts do not possess an evident coordinated vertical organization (Fig. 5j; Supplementary Fig. 5b). To investigate a possible genetic interaction between PCP and Wnt pathway genes during the establishment of support cell organization, we asked whether the support cell phenotype in Wnt pathway mutants would disrupt the support cell alignment in PCP mutants. Double vangl2;MZwnt11 (wnt11f1) homozygous mutants indeed show a loss of alignment in primII-derived neuromasts and normal, horizontal alignment of support cells in primI neuromasts as characteristic for single MZwnt11 (wnt11f1) mutants (Fig. 5k, l). This result shows that the wnt11 (wnt11f1) phenotype in support cells is epistatic and disrupts normal support cell alignment in PCP mutants.

To test if the support cell phenotype in wnt11 (wnt11f1) mutants is secondary to the hair cell phenotype or vice versa we prevented hair cell development in wild type and wnt11 (wnt11f1) mutants by depleting the hair cell specifying transcription factor atoh1a63 by CRISPR/Cas9-mediated genome editing (Supplementary Fig. 5c, d). While the uninjected wild-type siblings possess functional hair cells that can be labeled with the actin-binding protein β-II-Spectrin (Fig. 5m, n; Supplementary Fig. 5e), wild-type atoh1a CRISPants show no hair cells (Fig. 5o, p). In atoh1a CRISPants support cells are still normally aligned (Fig. 5o, p). Thus, support cell alignment is independently regulated from hair cells. Furthermore, MZwnt11 (wnt11f1) mutants injected with atoh1a CRISPR still show loss of support cell alignment in primII-derived neuromasts (Fig. 5q, r). Thus, the disorganization of support cell orientation observed in primII neuromasts of Wnt pathway genes is not a consequence of the hair cell misorientation. Altogether, these results indicate that, while vangl2 and scrib are not required for support cell alignment, the Wnt pathway genes are essential for the proper coordinated organization of support cells in primII-derived neuromasts.

Wnt pathway genes likely act in the premigratory primordium

Because wnt11 (wnt11f1) is not expressed in 5 dpf primII neuromasts, which show a phenotype in MZwnt11 (wnt11f1) mutants (Figs. 1 and 5), we hypothesized that wnt11 (wnt11f1) might be required earlier in lateral line development to establish hair cell orientation. We tested if Wnt pathway members are expressed in primII or in adjacent tissues during migration or placode specification stages. At 50 hpf, while primII is migrating and has not yet deposited its first neuromast, vangl2 is expressed in primII, and in primI and primII-derived neuromasts, suggesting that it is acting within lateral line cells (Fig. 6a). Likewise, the other PCP gene scrib is detected in the lateral line by in situ hybridization, agreeing with a previous RNA-Seq analysis64 (Fig. 6b). In contrast to vangl2, wnt11 (wnt11f1) mRNA is not detectable in either the migrating primordia, or primI-derived neuromasts (Fig. 6c). However, it is expressed in the underlying muscle along the myoseptum20,65, suggesting that the muscle could signal to the neuromasts (Fig. 6d; Supplementary Fig. 6a). In contrast to the wnt11 (wnt11f1) ligand, the Wnt co-receptor gpc4 is expressed in the migrating primII and primI-and primII-derived neuromasts, even though its loss only affects primII-derived neuromasts (Fig. 6e, Fig. 1). The expression of the fzd7a and fzd7b receptors is more complex. Both are expressed in the lateral line, but while fzd7a is expressed in primII, and primII-derived neuromasts (Fig. 6f), fzd7b is not expressed in primII but is expressed in primI-derived neuromasts (Fig. 6g). As only fzd7a is expressed in the migrating primII but only fzd7a/7b double mutants affect primII-derived neuromasts, we hypothesize that Wnt signaling is already acting during premigratory stages.

Fig. 6

Temporal dynamic expression of the PCP and Wnt pathway genes during formation and migration of primII. ag In situ localization on 50 hpf wild-type fish of mRNA for vangl2 (a), scrib (b), and wnt11 (wnt11f1) (c), at the level of the primordium; (d), at the level of the underlying muscle), gpc4 (e), fzd7a (f), fzd7b (g). The first neuromast derived from primI is outlined using black, while primII is outlined in white in (ag). h In situ localization of wnt11 (wnt11f1) mRNA in a 34 hpf wild-type embryo. i Magnification of the expression in the area posterior to the ear in (h). The ear is delimited by a dashed line. j In situ localization of gpc4 mRNA in the area posterior to the ear at 32 hpf. Arrowhead indicates the putative localization of the D0 placode. kn Still frames of the time lapse analysis of the formation of primII, primD, occipital prim, and D1 labeled in a Tg(cldnb:lynGFP) transgenic wild-type fish (Supplementary Video 5). Arrow in k indicates the original group of cells that gives rise to all three primordia. Arrowheads in ln indicate the different primordia formed. Asterisk in m, n indicates the position of the D1 neuromast. o, p Schematic cartoon of the proposed mechanism by which Wnt11 (Wnt11f1) signals to cells in the D0 placode (o) to establish support cell organization (p). q t-SNE plots and violin plots showing expression of fzd7b (q) and vangl2 (r) in a 5 dpf neuromast during homeostasis. The Wilcox p-value for q = 8.45 × 10−32 in support cells and mantle cells versus hair cells, while in r the expression pattern was too sparse to generate meaningful statistics. HCs hair cells, SCs support cells, MCs mantle cells. *** denotes statistical significance. Scale bar in a equals 10 μm, h equals 50 μm, i equals 25 μm, k equals 50 μm

Analysis of the expression pattern of the Wnt pathway genes at a time point in which primII is being specified (32 hpf) shows that wnt11 (wnt11f1) is expressed in a dispersed group of cells posterior to the ear immediately adjacent to the forming, gpc4-expressing D0 placode (Fig. 6h-j arrowhead). In addition, wnt11 (wnt11f1) is expressed in the lens, brain, ear and dorsal spinal cord. The D0 placode gives rise to primII, primD (that gives rise to the dorsal lateral line)25,34 and the occipital prim (occipital lateral line) (Fig. 6j arrowhead).

Time-lapse analysis of the formation of primII in wild type embryos shows how primII, primD and the occipital prim arise from the D0 placode between 24 and 48 hpf (Fig. 6k–n; Supplementary Movie 5). Neuromasts in all these three lateral lines possess the same D-V hair cell orientation in wild-type embryo (Supplementary Fig. 6c), and also show concentric hair cell organization in the Wnt pathway mutants (Supplementary Fig. 6c). Due to the fact that the neuromasts derived from primD and the occipital prim do not migrate over any wnt11 (wnt11f1)-expressing muscle cells, unlike primII in the trunk, we conclude that the hair cell defect in primII neuromasts is not due to loss of Wnt signaling from muscle cells along the horizontal myoseptum. The only time these three lateral lines are all exposed to wnt11 (wnt11f1) is when they arise from D0, suggesting that wnt11 (wnt11f1) is required in the placode before the three primordia migrate into different directions (Fig. 6o, p).

Single-cell RNA-sequencing (scRNA-Seq) analysis of neuromasts also suggests that the Wnt pathway genes act in support cells, rather than hair cells66. gpc4 and fzd7a/b are robustly expressed in support cells but downregulated as cells differentiate into hair cells (Fig. 6q; Supplementary Fig. 6b). vangl2 and scrib are expressed in both support and hair cells (Fig. 6r; Supplementary Fig. 6b), however, the loss of vangl2 only affects the hair cells. The role of vangl2 in support cells is therefore still unresolved.

Overall, these results suggest that while PCP genes are expressed and required to establish proper hair cell planar polarization within all neuromasts, Wnt pathway genes act earlier in support cells during D0 placode formation, prior to the differentiation of hair cells. Support cells then secondarily influence hair cell orientations in 5 dpf primII neuromasts (Fig. 6p, q). Thus, the loss of Wnt signaling early in development has effects on organ formation several days later.


PCP and Wnt pathway genes are involved in the establishment of hair cell orientation in vertebrates23,24,54,55,56,67,68,69,70,71. Because disruptions of both pathways cause hair cell arrangement defects, Wnt pathway mutants are often classified as PCP mutants. Wnt ligands play different roles in different PCP contexts. For example, Wnt ligands instruct PCP15,16,17,44 or act as gradients that control hair cell orientation in the inner ear23,24. Our results demonstrate that in the context of neuromasts, the Wnt pathway genes wnt11 (wnt11f1), gpc4 and fzd7a/7b do not affect PCP signaling as Vangl2 localization is normal in Wnt pathway mutants (Fig. 3). In addition, in MZwnt11 (wnt11f1);vangl2 double homozygous neuromasts, hair cell orientations are randomized as in vangl2 mutants, suggesting that PCP signaling is normal in MZwnt11 (wnt11f1) mutants (Fig. 2). Recent reports show that Emx2 and Notch signaling control stereocilia bundle orientation and that Vangl2 is normally localized in emx2 mutants suggesting that this pathway acts in parallel to the PCP pathway36,72. As emx2 affects hair cell polarity without affecting PCP signaling, we wondered if the Wnt pathway genes acted in concert with Emx2 or Notch signaling. However, the number of Emx2-expressing hair cells is normal in MZwnt11 (wnt11f1), even though they are not localized to one half of the neuromasts but are randomly distributed (Supplementary Fig. 7a–e). Therefore, Wnt pathway genes are not acting in the same pathway with Notch and Emx2 signaling to regulate hair cell orientation. Instead, our data suggest that Wnt pathway genes act in emx2-negative support cells, whose misalignment causes hair cell orientation defects secondarily in the absence of Wnt signaling.

An unresolved question is why in Wnt pathway mutants the concentric hair cell phenotype arises sequentially as more cells are added. A concentric orientation might represent the most energy-efficient arrangement for hair cells that still possess functional PCP but that are surrounded by misaligned support cells. Our results stress the importance of studying all cell types in an organ when analyzing hair cell phenotypes in vertebrates. Therefore, gpc4 and MZfz7a/7b mutants previously characterized as PCP signaling mutants in other contexts should be re-evaluated as such.

How are the different orientations in primI and primII-derived neuromasts achieved? PCP pathway mutations disrupt hair cell orientations in all neuromasts. Thus, the mechanisms that control differential A-P and D-V orientations in primI and primII-derived neuromasts are either acting upstream or in parallel to PCP signaling. Lopez-Schier et al.37 proposed that the direction of the migrating primordia or the recently deposited neuromasts determines the axis of polarity. Neuromasts deposited by primII migrate ventrally after deposition32,73, which has been correlated with instructing the axis of hair cell polarity with a 90° angle with respect to primI-derived neuromasts. However, the adjacent primI-derived interneuromast cells also undergo a ventral migration and form neuromasts with primI-polarity25. Likewise, the D1 neuromast forms from cells left behind by primI and possesses primI polarity (Supplementary Fig. 6c), even though it undergoes a dorsal migration after being formed25. Therefore, the direction of migration is not an indicator of hair cell polarity. Our data suggest that support cell polarity in different primordia is set up as they are formed, and which instructs hair cell polarity in later forming neuromasts.

Wnt pathway genes are only required for support cell organization in primII- and not primI-derived neuromasts (Fig. 5) raising the question of how primI-derived neuromasts are polarized. Support cells in primI neuromasts could be organized by a mechanism that involves tissue tension as described in the skin of mouse74, ciliated epithelia of Xenopus75,76 and in Drosophila77,78. Alternatively, primI-derived neuromasts may rely on a different subset of Wnt ligands, HSPGs or Fzd receptors to organize their support cells79,80. To date, the analysis of hair cell orientation in zebrafish mutations in two noncanonical Wnt ligands, wnt5b (pipetail) and wnt11f2 (formerly known as wnt11/silberblick40), revealed no hair cell orientation defects in any primordia (Supplementary Figs. 1 and 7f).

Our data suggest that tissue organization in the primordium is set up early during development and influences hair cell orientation in later stages. This mechanism is conceptually analogous to the ratchet effect proposed by Gurdon et al.81 and implies that cells have a memory of the initial conditions or signals to which they have been exposed that modulates a later response. A similar process is at work during zebrafish gastrulation, where prolonged cadherin-dependent adhesion initiates Nodal signaling and feeds back to positively increase adhesion and determines mesoderm vs. endoderm fate82. In addition, reports from cells remembering the spatial geometry or PCP that precedes cell division using the extracellular matrix or tricellular junctions support this hypothesis83,84,85. The memory of early polarity establishment might explain why primII-derived Wnt pathway mutant neuromasts possess a phenotype, even though wnt11 (wnt11f1) is not expressed in surrounding tissues at that stage (Figs. 1 and 5).

Rather than acting as an instructive cue, Wnt pathway genes might be acting as permissive factors by controlling cell–cell adhesion. wnt11 (wnt11f1) destabilizes apical cell–cell junctions in the epithelium during pharyngeal pouch formation in zebrafish86, and expression of dominant-negative Wnt11 in Xenopus shows that Wnt11 controls cell adhesion through cadherins87. Interestingly, wnt11f2 interacts with gpc4 and fzd7a/7b and influences E-cadherin-dependent cell–cell adhesion, rather than PCP during zebrafish CE and eye formation19,50,88. However, even though wnt11 (wnt11f1) binds to the same receptors as wnt11f2, wnt11f2 does not affect hair cell development, suggesting that the two wnt11 orthologs likely control different adhesion molecules in the different tissues.

Another intriguing possibility is that the Wnt pathway genes might act through the Fat-Dachsous (Ft-Ds) pathway. In flies, disruptions in Ft-Ds signaling cause swirling wing hair patterns and disruptions of the global alignment of PCP proteins without affecting their asymmetric distribution, reminiscent of the phenotypes we observed in Wnt pathway mutants3,6,89,90,91,92. Furthermore, a recent report shows that the Ft-Ds pathway directs the uniform axial orientation of cells in the Drosophila abdomen93, which may be similar to the coordinated organization observed in support cells in our study. It is likely that wnt11 (wnt11f1), gpc4 and fzd7a/7b establish support cell organization by controlling their adhesive properties. However, the presence of a large number of adhesion molecules, and potential for functional compensation, makes functional analyses challenging.

In summary, we identified and characterized the Wnt pathway genes wnt11 (wnt11f1), gpc4 and fzd7a/7b, and the PCP gene scrib as distinct inputs controlling hair cell orientation in the lateral line of zebrafish. The core PCP components vangl2 and scrib control individual hair cell polarity, while the Wnt pathway genes wnt11 (wnt11f1)/gpc4/fzd7a/7b affect the alignment of support cells, which are the progenitors of the later forming hair cells (Fig. 7). This interpretation is supported by our findings that PCP mutants show hair cell orientation defects in the presence of normally aligned surrounding support cells. Conversely, in Wnt pathway mutants support cells are misaligned, even in the absence of hair cells. Importantly, scRNA-Seq analysis of neuromasts shows that gpc4, fzd7a and fzd7b are robustly expressed in support but not hair cells, whereas vangl2 is also strongly expressed in hair cells. In addition, because the affected support cells in Wnt pathway mutants are only exposed to wnt11 (wnt11f1) ligand while the primordia are still in the head region, we propose that Wnt pathway genes act early during development before the hair cells appear.

Fig. 7

The PCP and Wnt pathways act in parallel to establish coordinated hair cell polarity and orientation in the neuromast. Model of how the PCP signaling genes Vangl2 and Scrib are required to establish individual polarity in the hair cells (left part of the box), while the Wnt pathway members Wnt11 (Wnt11f1), Gpc4 and Fzd7a/7b interact to establish coordinated support cell alignment (right part of the box) in primII-derived neuromasts. The coordinated alignment of support cells, which we assume have normal polarity because coordinated alignment is not disrupted in PCP signaling mutants, then dictates the individual hair cell orientation

Our study provides an alternative mechanistic model in which hair cell orientation defects are not only caused by disruptions of the PCP pathway but independently also by other pathways, such as Wnt11 (Wnt11f1)-activated Wnt signaling. The precise molecular mechanism by which Wnt signaling affects hair cell orientation is unknown but it possibly affects adhesion between support cells required to establish or maintain hair cell alignment.


Fish husbandry

This study was conducted in accordance with the recommendations in the Guide for the Care and Use of Laboratory Animals of the NIH and a protocol approved by the Institutional Animal Care and Use Committees of the Stowers Institute (TP Protocol: # 2017-0176).

All experiments were performed per guidelines established by the Stowers Institute IACUC review board. The following mutant fish strains previously described were used: trim209 94, gpc4fr6 45, wnt11 (wnt11f1)fh224(wnt11rfh224 in95), wnt11f2tz216(wnt11/slb in96) fzd7ae3 and fzd7bhu3495 97, scribrw468 98, wnt5bti265 58.

The following transgenic fish lines were used: Tg(cldnb:lynGFP)zf106 99, Tg(myo6b:β -Actin-GFP)100, Tg(cxcr4b:H2A-EGFP)101, Et(krt4:EGFP)sqET4 and Et(krt4:EGFP)sqET20 102, Tg(cldnB:H2A-mCherry)psi4 103.

In situ hybridization

Samples were fixed in 4% PFA overnight at 4 °C. Samples were then dehydrated in PBS/Tween 0.3% (PBSTw) and a Methanol series (0, 25, 50, 75 and 100%) for 10 min/each and kept overnight at −20 °C in 100% Methanol. Then, embryos were rehydrated in PBSTw and a Methanol series and incubated with Proteinase K (10 µg/mL in PBSTw) for 2 min at RT. The fish were then postfixed in 4% PFA in PBS for 30 min. After postfixation, the larvae were incubated in Hybridization mix for 2 h at 65 °C, and then were hybridized with the Probes overnight at 65 °C. The following day the unbound probes was removed using a series of washes (50% Formamide/50% 2× SSC; 50% Formamide/5× SSC/0.25% CHAPS (Hyb Wash); 50% Hyb wash/50% 2× SSC; 25% Hyb wash/75% 2× SSC; 2× SSC/0.25% CHAPS; 0.2 SSC/0.25% CHAPS; PBSTw/0.25% CHAPS; 100 mM Maleic Acid/50 mM NaCl pH adjusted to 7.5 (MAB); MAB/0.1% Tween) using an Intavis InSituPro robot and detected with an alkaline phosphatase-bound anti-DIG Fab fragment (Roche) (1:4000 in MABT + 10% NGS + 1 mg/mL BSA). Colorimetric development was performed using nitrotetrazolium blue (NBT) and bromochloroindoyl phosphate (BCIP)104,105. The following probes were used: wnt11 (wnt11f1) (called wnt11r in65), gpc4106, fzd7a and fzd7b107. The vangl2 probe was generated using the following pair of Fw/Rv primers (TCATCTCAGAAGCGATCCAGTA/CCACATGCATCAGACCTAAAAA), the scrib probe was generated using the following pair of Fw/Rv primers (AGGATCTTGCCAAGCAAGTG/CCCTGGCGTAGTTTACGTTT), and the vangl1 probe was generated using the following pair of Fw/Rv primers (AGCCCTGCTTCTCTCTATGTGT/CAAACTTGTGTGATTTGGGATG) from wild-type AB DNA.

Immunohistochemistry and Phalloidin staining

For β-II-Spectrin, ZO-1 and Vangl2 antibody stainings, embryos were fixed in 2% trichloroacetic acid (TCA) in water at room temperature for at least 4 h. Embryos were then washed briefly in 0.5% Triton-X in PBS (PBSTx) and then blocked for 2 h in PBSTx + 2% normal goat serum (NGS). Primary antibodies Rabbit anti-Vangl2 (1:100, Anaspec, AS-55659s, now discontinued), Mouse anti ZO-1 (1:200, Invitrogen #339100), Mouse anti β-II-Spectrin (1:200, BD Transduction, 612562) were diluted in Blocking solution and incubated overnight at 4 °C. Primary antibody was washed using PBSTx and then detected using either Alexa-568 Anti-Rabbit and Alexa-488 Anti-Mouse Secondary antibodies for the double β-II-Spectrin/Vangl-2; or Alexa-594 Anti-Mouse (Thermo Fisher) for the double β-II-Spectrin/ZO-1 diluted 1:500 in Blocking Solution, and incubated overnight at 4 °C. Secondary antibody was washed thoroughly the next day using PBSTx before imaging.

For Emx2 immunolabeling 5 dpf embryos were fixed in 4% PFA overnight at 4 °C. Then, embryos were permeabilized in acetone for 5 min at −20 °C and incubated with Blocking Solution (2% NGS, 1% BSA in PBS) for 2 h. Fish were then incubated with primary antibody (rabbit anti-Emx2, K0609; Trans Genic, Japan; 1:250) overnight at 4 °C. The following day, fish were washed in 1× PBS and incubated with the secondary antibody (1:250 in Blocking Solution) for 2 h at RT. The fish were then washed thoroughly in PBS and imaged72.

For Phalloidin staining, embryos were fixed in 4% PFA in 1× PBS at room temperature for at least 2 h. PFA-fixed embryos were briefly washed in 0.5% Triton-X in 1× PBS and then permeabilized in 2% PBSTx for 2 h at room temperature. Subsequently, the embryos were stained with Alexa Fluor 488 Phalloidin (Thermo Fisher; 1:40 in PBSTx 0.5%) for 2 h. After staining, the embryos were washed thoroughly using PBSTx 0.5% and imaged.

Neomycin treatment

To kill hair cells, 5 dpf embryos were treated with 300μM Neomycin in 0.5 E2 media for 30 min62. Neomycin was then washed away using fresh E2 media, and waited 3 h before fixation in 4% PFA in 1× PBS.

Time-lapse imaging and in vivo imaging

Embryos were anesthetized with Tricaine (MS-222) and mounted in 0.8% low-melting point agarose in glass bottom dishes (MatTek, USA). Embryos were imaged with a Zeiss 780 confocal microscopes using a 40×/1.1 W Corr M27 objective in a climate-controlled chamber set to 28 °C27.

Hair cell orientation analysis

To calculate the hair cell orientation from the Phalloidin-stained neuromasts, the Line tool from FIJI108 was used. A straight line was drawn from the pole opposite to the kinocilium towards the pole were the kinocilium was found. To create the Rose diagrams to represent hair cell orientation, angles measured and then plotted using the rose.diag() function in R ggplot. Statistical analysis was performed for each condition against wild type using Fisher’s exact test. To determine A-P or D-V binomial distribution, the data are binned to four groups, left, right, bottom, and up. The binomial test is used to test whether ‘right + left’ counts are different from 50% of total counts.

Measure of hair cell alignment and concentricity

We must choose a structure against which to compare the cell’s angles. Specifically, we are looking at relative differences in the angles and an assumed underlying arrangement, rather than comparing them to some absolute feature, such as the horizontal. The first comparison we consider is the angular difference between nearest neighbors. Note although it is possible to provide a consistent polarization of the cell and, thus, measure the angle between two nearest major axes on a scale of (−180, 180)° we are not currently interested in the polarization, thus, we always take the smallest angle between the two major axes. Hence, the angles will be on a scale of (−90, 90)°. Further, the sign convention we will be using is positive if the angle measured from the current cell is anticlockwise, and negative otherwise. The second comparison we consider is cell alignment when compared to a fitted ellipse. Initially, we take the cell centers of the Lines calculated in the “Hair cell orientation analysis” section, and use a least squares fitting algorithm based on principal component analysis to create an ellipse of best fit. Each cell is then projected to the closest point on the fitted ellipse’s boundary and their major axis angle is compared to that of the ellipse’s tangent at the nearest point. The smallest angle is extracted using the above sign rule. The “Nearest neighbor measurement” provides us with a measurement of how aligned each cell is with its neighbors, while the “Nearest tangent measurement” will provide us with a measurement of how aligned each cell is with the fitted ellipse. Specifically, this comparison will suggest whether there is a circular structure underlying the cell alignment. Having derived the data from the experimental results we plot the information as a histogram. Specifically, the range (−90, 90)° is divided up into 12 bins and we tally how often each angle falls within one of these bins. Dividing by the total number of results then normalizes the histograms to represent a probability. Each angle distribution was first tested against the null hypothesis that there was no preferred direction. Thus, we compare the probability histogram against the uniform distribution and see if there was a significant difference, namely p < 0.01. If there was a significant difference we then compared the solutions to the Von Mises distribution, which is the generalized Normal distribution that is periodic on the angular domain. The fitting of the Von Mises distribution tells us if there is a preferred direction and how variable the alignment is. The code for these analyses is publicly available at https://github.com/ThomasEWoolley/Cell_alignment.

Vangl2 asymmetry quantification

Vangl2 asymmetry quantifications from immunolabeled embryos were performed from raw images. Upon visual inspection, Vangl2 being “asymmetric” vs. “not being asymmetric” was assigned and quantified using the Cell Counter function of FIJI. Fisher’s exact test was performed to determine statistical differences between samples. From the hair cells that showed Vangl2 asymmetry, a second analysis was performed and classified into three categories: we quantified whether the enrichment was (1) in the pole where the kinocilium is, (2) on the opposite pole, or (3) enriched but out of the axis determined by the kinocilium. Fisher’s exact test was performed to determine statistical differences between samples. The double immunolabeling images were processed for contrast and sharpness only for visual display in the Figure afterwards using Photoshop CS6.

Generation of the Tg(myo6b:GFP-XVangl2) construct

GFP-XVangl2 was amplified from pDest2-GFP-Vangl2 plasmid (A kind gift from J Wallingford109) and Topo TA cloned. The Topo vector was then digested using KpnI and SacI, and ligated into the KpnI-SacI sites of the Tol2 middle entry vector110 using Quick ligase (NEB). The middle entry GFP-XVangl2 vector was recombined via a Gateway reaction with the 5′ myo6b vector100. The final myo6b:GFP-XVangl2 plasmid was co-injected into AB or MZwnt11 (wnt11f1) mutant embryos together with Tol2 Transposase mRNA at a final concentration of 30 ng/µl.

GFP-XVangl2 profile analysis

Images were acquired in a Zeiss 780 microscope using a 40×/1.1 W Corr M27 objective. Raw images of Phalloidin-stained animals were used for the analysis of GFP intensity. GFP-XVangl2 polarity was determined in a manner analogous to111. These utilized custom plugins as described above. Average cortical line profiles were generated with a 4 pixel thickness utilizing the “polyline kymograph jru v1” plugin. Then maximum angular position of intensity was determined using the “trajectory statistics jru v2” plugin. Profiles were then aligned so that the maximum intensity occurred at angle 0 with “set multi plot offsets jru v1”. Next, angles were wrapped to values between −179 and +180 degrees with “wrap angle profile jru v1”. Finally, profiles were averaged with “average trajectories jru v1” (available at http://research.stowers.org/imagejplugins/) with error bars indicating the standard error in the mean. For some presentations, averaged profiles were normalized to a maximum intensity of 1 for comparison purposes. Peak widths were determined by fitting profiles to a Gaussian peak function via nonlinear least squares fitting (plugin is “fit multi gaussian jru v1”) with error bars determined by fitting 100 Monte Carlo simulated random data sets112. Polarity ratios were determined by averaging three values surrounding the 0°, 90°, and 180° data points and calculating their ratios with errors propagated according to ref. 112.

Hair cell progenitor angle of division analysis

Imaging was performed in a Zeiss 780 using a 40×/1.1W Corr M27 objective, under conditions described above (Time-lapse imaging section). To obtain a quantitative measurement of how hair cell progenitors divide within the neuromast, we acquired time-lapses of migrating primII in wild type and MZwnt11 (wnt11f1) mutant embryos in a tg(cxcr4b:H2A-EGFP); tg(myo6b:β -Actin-GFP) double background, scanning every 5 min. We calculated the division angle of the dividing progenitor with respect to the radius from the center of division, to the center of the neuromast.

We used Imaris ×64 9.2.1 to manually mark the location of all cell divisions and the center point of the depositing neuromast for all timepoints. To find the center of the neuromast we create a Surface object using the H2A-EGFP channel with very coarse surface detail (surface grain size ~ 20 µm). For each cell division, we used Spots to manually mark the center of each daughter hair cell. The Surface and Spots data for every timepoint is exported and aggregated in an Excel spreadsheet. With the exported data in Excel, we calculated two vectors for every dividing cell pair. We calculated the vector between each of the daughter cells, as well as the vector from the center of the neuromast to the center of cell division. The smallest angle between the two vectors is calculated to give the division angle with respect to the radius, which is the range from 0° to 90°. Division angles for Wild type and mutant were then plotted and t -test analysis analysis performed to calculate statistical differences between wild type and MZwnt11 (wnt11f1) mutants.

Support cell orientation analysis

To obtain the support cell orientation, Phalloidin-stained or ZO-1-stained neuromasts were processed in FIJI108. A custom “gray morphology jru v1” plugin (available at http://research.stowers.org/imagejplugins/) was used to sharpen the signal from the cell membranes and afterwards segmented using the MorphoJ plugin113. Once a mask of the cells within the neuromast was obtained, we found the orientation of each cell using FIJI’s “Analyze Particles” function. This function fits each cell to an ellipse in order to provide spatial data, including the center point, major and minor axis length, and the major and minor axis angle in cartesian coordinates. We exported the data from FIJI to Python where we processed and plotted the data. We used Matplotlib to create a histogram of the distribution of cell orientation angles in the range of 0°–90°. To visualize and verify the data, we also plotted the major axis vector on top of the cell mask image for each sample. The code for this analysis is publicly available at https://github.com/richard-alexander/neuromast_cell_orientation.

vangl1 CRISPR

We designed two guide RNAs using CRISPRscan (www.crisprscan.org)114 targeting exon 3 of vangl1 (ENSDARG00000004305). The guide-RNA plus PAM sequences are 5′-GGTTCCAGTGACCGCCGTGGTGG-3′ and 5′-GGCTTTGGGAAGGACACGGAGGG-3′ in vitro transcription using a MEGAShortscript T7 kit(Invitrogen) was carried out the manufacturer’s recommended conditions. RNA was purified using an RNA Clean-up and Concentrator kit (Zymo Research). One-cell stage embryos were injected with an injection mixture containing 1 μg of Cas9-NLS Protein (PNABio) with 170 ng of each guide-RNA. To assess cutting efficiency, the region around the cutting sites was amplified from genomic-DNA by PCR using GGAGACCTGGGTACTTCCAT and TTAGCAGATCTCATCAAGAACA as primers using GoTaq Master Mix (Promega) and run on an agarose gel.

atoh1a CRISPR

To target atoh1a (ENSDARG00000055294), CHOPCHOP tool115 was used to design the target sites. The protocol described in116 was followed to generate two guide RNAs targeting atoh1a’s single exon. The generic DNA Oligo B AAAAGCACCGACTCGGTGCCACTTTTTCAAGTTGATAACGGACTAGCCTTATTTTAACTTGCTATTTCTAGCTCTAAAAC was annealed with DNA oligos possessing a T7 promoter plus atoh1a’s coding regions 5′-TAATACGACTCACTATAGGCTGGCTCCCGTGCAGGCGTTTTAGAGCTAGAAATAGC-3′ and 5′-TAATACGACTCACTATAGGGAGAGGCGAAGAATGCAGTTTTAGAGCTAGAAATAGC-3′ and amplified by PCR. From the resulting DNA template, the in vitro reaction was carried out with the T7 MEGAshortscript kit (Invitrogen) under manufacturer conditions, and the RNA was purified and concentrated using the RNA Clean & Concentrator-25 kit (Zymo, #R1017). A mixture of 30 ng of each gRNA was mixed with 1 μg of recombinant Cas9-NLS protein (PNA BIO, CP04-100) and injected into one-cell stage embryos. To assess the success of the injections, 5 dpf CRISPant embryos were stained with DASPEI (2-(4-(dimethylamino)styryl)-N-ethylpyridinium iodide, [Invitrogen, USA]) diluted in embryo media and screened for the lack of hair cells compared with the uninjected siblings. To assess cutting efficiency, the region around the cutting sites was amplified from genomic-DNA by PCR using ATGGATGGAATGAGCACGGAT and AGTTTCAGTTCCGACAGCTCG as primers and run on an agarose gel.

Single-cell RNA-Seq

The scRNA-Seq has been described in detail in66. The BAM files and count matrices produced by cell ranger can be accessed in the Gene Expression Omnibus (GEO) database (accession number GSE123241).

Together with this paper we published a publicly available, fully searchable database that allows the user to determine in which neuromast cell type candidate genes are expressed: https://piotrowskilab.shinyapps.io/neuromast_homeostasis_scrnaseq_2018/.

Reporting summary

Further information on research design is available in the Nature Research Reporting Summary linked to this article.

Data availability

The authors declare that all data supporting the findings of this study are available within the article and its supplementary information files or from the corresponding author upon reasonable request. The source data underlying Figs. 1,2,3,4 and Supplementary Figs. 2, 4 and 7 are provided as a Source Data file. Uncropped blots for Supplementary Figs. 2 and 5 are also provided in the Source data file. This has also been deposited in the Stowers Institute Original Data Repository and available online at http://www.stowers.org/research/publications/libpb-1424.


  1. 1.

    Goodrich, L. V. & Strutt, D. Principles of planar polarity in animal development. Development 138, 1877–1892 (2011).

  2. 2.

    Butler, M. T. & Wallingford, J. B. Planar cell polarity in development and disease. Nat. Rev. Mol. Cell Biol. 18, 375–388 (2017).

  3. 3.

    Devenport, D. The cell biology of planar cell polarity. J. Cell Biol. 207, 171–179 (2014).

  4. 4.

    Strutt, H. & Strutt, D. Long-range coordination of planar polarity in Drosophila. Bioessays 27, 1218–1227 (2005).

  5. 5.

    Lawrence, P. A. & Shelton, P. M. The determination of polarity in the developing insect retina. J. Embryol. Exp. Morphol. 33, 471–486 (1975).

  6. 6.

    Gubb, D. & Garcia-Bellido, A. A genetic analysis of the determination of cuticular polarity during development in Drosophila melanogaster. J. Embryol. Exp. Morphol. 68, 37–57 (1982).

  7. 7.

    Wong, L. L. & Adler, P. N. Tissue polarity genes of Drosophila regulate the subcellular location for prehair initiation in pupal wing cells. J. Cell Biol. 123, 209–221 (1993).

  8. 8.

    Lawrence, P. A. Development and determination of hairs and bristles in the milkweed bug, Oncopeltus fasciatus (Lygaeidae, Hemiptera). J. Cell Sci. 1, 475–498 (1966).

  9. 9.

    Tada, M. & Smith, J. C. Xwnt11 is a target of Xenopus Brachyury: regulation of gastrulation movements via Dishevelled, but not through the canonical Wnt pathway. Development 127, 2227–2238 (2000).

  10. 10.

    Wallingford, J. B. et al. Dishevelled controls cell polarity during Xenopus gastrulation. Nature 405, 81–85 (2000).

  11. 11.

    Heisenberg, C. P. et al. Silberblick/Wnt11 mediates convergent extension movements during zebrafish gastrulation. Nature 405, 76–81 (2000).

  12. 12.

    Gao, B. Wnt regulation of planar cell polarity (PCP). Curr. Top. Dev. Biol. 101, 263–295 (2012).

  13. 13.

    Yang, Y. & Mlodzik, M. Wnt-Frizzled/planar cell polarity signaling: cellular orientation by facing the wind (Wnt). Annu. Rev. Cell Dev. Biol. 31, 623–646 (2015).

  14. 14.

    Humphries, A. C. & Mlodzik, M. From instruction to output: Wnt/PCP signaling in development and cancer. Curr. Opin. Cell Biol. 51, 110–116 (2018).

  15. 15.

    Wu, J., Roman, A. C., Carvajal-Gonzalez, J. M. & Mlodzik, M. Wg and Wnt4 provide long-range directional input to planar cell polarity orientation in Drosophila. Nat. Cell Biol. 15, 1045–1055 (2013).

  16. 16.

    Gros, J., Serralbo, O. & Marcelle, C. WNT11 acts as a directional cue to organize the elongation of early muscle fibres. Nature 457, 589–593 (2009).

  17. 17.

    Chu, C. W. & Sokol, S. Y. Wnt proteins can direct planar cell polarity in vertebrate ectoderm. eLife 5, e16463 (2016).

  18. 18.

    Witzel, S., Zimyanin, V., Carreira-Barbosa, F., Tada, M. & Heisenberg, C. P. Wnt11 controls cell contact persistence by local accumulation of Frizzled 7 at the plasma membrane. J. Cell Biol. 175, 791–802 (2006).

  19. 19.

    Ulrich, F. et al. Wnt11 functions in gastrulation by controlling cell cohesion through Rab5c and E-cadherin. Dev. Cell 9, 555–564 (2005).

  20. 20.

    Gordon, L. R., Gribble, K. D., Syrett, C. M. & Granato, M. Initiation of synapse formation by Wnt-induced MuSK endocytosis. Development 139, 1023–1033 (2012).

  21. 21.

    Deans, M. R. A balance of form and function: planar polarity and development of the vestibular maculae. Semin. Cell Dev. Biol. 24, 490–498 (2013).

  22. 22.

    May-Simera, H. & Kelley, M. W. Planar cell polarity in the inner ear. Curr. Top. Dev. Biol. 101, 111–140 (2012).

  23. 23.

    Dabdoub, A. et al. Wnt signaling mediates reorientation of outer hair cell stereociliary bundles in the mammalian cochlea. Development 130, 2375–2384 (2003).

  24. 24.

    Qian, D. et al. Wnt5a functions in planar cell polarity regulation in mice. Dev. Biol. 306, 121–133 (2007).

  25. 25.

    Ghysen, A. & Dambly-Chaudiere, C. The lateral line microcosmos. Genes Dev. 21, 2118–2130 (2007).

  26. 26.

    Pujol-Marti, J. & Lopez-Schier, H. Developmental and architectural principles of the lateral-line neural map. Front. Neural Circuits 7, 47 (2013).

  27. 27.

    Venero Galanternik, M., Navajas Acedo, J., Romero-Carvajal, A. & Piotrowski, T. Imaging collective cell migration and hair cell regeneration in the sensory lateral line. Methods Cell Biol. 134, 211–256 (2016).

  28. 28.

    Fritzsch, B. & Straka, H. Evolution of vertebrate mechanosensory hair cells and inner ears: toward identifying stimuli that select mutation driven altered morphologies. J. Comp. Physiol. A Neuroethol. Sens. Neural Behav. Physiol. 200, 5–18 (2014).

  29. 29.

    Chagnaud, B. P., Engelmann, J., Fritzsch, B., Glover, J. C. & Straka, H. Sensing external and self-motion with hair cells: a comparison of the lateral line and vestibular systems from a developmental and evolutionary perspective. Brain Behav. Evol. 90, 98–116 (2017).

  30. 30.

    Piotrowski, T. & Baker, C. V. The development of lateral line placodes: taking a broader view. Dev. Biol. 389, 68–81 (2014).

  31. 31.

    Gompel, N. et al. Pattern formation in the lateral line of zebrafish. Mech. Dev. 105, 69–77 (2001).

  32. 32.

    Ledent, V. Postembryonic development of the posterior lateral line in zebrafish. Development 129, 597–604 (2002).

  33. 33.

    Metcalfe, W. K., Kimmel, C. B. & Schabtach, E. Anatomy of the posterior lateral line system in young larvae of the zebrafish. J. Comp. Neurol. 233, 377–389 (1985).

  34. 34.

    Nunez, V. A. et al. Postembryonic development of the posterior lateral line in the zebrafish. Evol. Dev. 11, 391–404 (2009).

  35. 35.

    Ji, Y. R., Warrier, S., Jiang, T., Wu, D. K. & Kindt, K. S. Directional selectivity of afferent neurons in zebrafish neuromasts is regulated by Emx2 in presynaptic hair cells. eLife 7, e35796 (2018).

  36. 36.

    Jacobo, A., Dasgupta, A., Erzberger, A., Siletti, K. & Hudspeth, A. J. Notch-mediated polarity decisions in mechanosensory hair cells. Preprint at bioRXiv https://doi.org/10.1101/480798 (2018).

  37. 37.

    Lopez-Schier, H., Starr, C. J., Kappler, J. A., Kollmar, R. & Hudspeth, A. J. Directional cell migration establishes the axes of planar polarity in the posterior lateral-line organ of the zebrafish. Dev. Cell 7, 401–412 (2004).

  38. 38.

    Lopez-Schier, H. & Hudspeth, A. J. A two-step mechanism underlies the planar polarization of regenerating sensory hair cells. Proc. Natl Acad. Sci. USA 103, 18615–18620 (2006).

  39. 39.

    Mirkovic, I., Pylawka, S. & Hudspeth, A. J. Rearrangements between differentiating hair cells coordinate planar polarity and the establishment of mirror symmetry in lateral-line neuromasts. Biol. Open 1, 498–505 (2012).

  40. 40.

    Postlethwait, J. H., Navajas Acedo, J. & Piotrowski, T. Evolutionary Origin and Nomenclature of Vertebrate Wnt11-Family Genes. Zebrafish https://doi.org/10.1089/zeb.2019.1760 (2019).

  41. 41.

    Bradley, E. W. & Drissi, M. H. Wnt5b regulates mesenchymal cell aggregation and chondrocyte differentiation through the planar cell polarity pathway. J. Cell Physiol. 226, 1683–1693 (2011).

  42. 42.

    Wada, H. & Okamoto, H. Roles of planar cell polarity pathway genes for neural migration and differentiation. Dev. Growth Differ. 51, 233–240 (2009).

  43. 43.

    Wada, H. & Okamoto, H. Roles of noncanonical Wnt/PCP pathway genes in neuronal migration and neurulation in zebrafish. Zebrafish 6, 3–8 (2009).

  44. 44.

    Gao, B. et al. Wnt signaling gradients establish planar cell polarity by inducing Vangl2 phosphorylation through Ror2. Dev. Cell 20, 163–176 (2011).

  45. 45.

    Topczewski, J. et al. The zebrafish glypican knypek controls cell polarity during gastrulation movements of convergent extension. Dev. Cell 1, 251–264 (2001).

  46. 46.

    Roszko, I., D, S. S., Jessen, J. R., Chandrasekhar, A. & Solnica-Krezel, L. A dynamic intracellular distribution of Vangl2 accompanies cell polarization during zebrafish gastrulation. Development 142, 2508–2520 (2015).

  47. 47.

    Ohkawara, B., Yamamoto, T. S., Tada, M. & Ueno, N. Role of glypican 4 in the regulation of convergent extension movements during gastrulation in Xenopus laevis. Development 130, 2129–2138 (2003).

  48. 48.

    Rochard, L. et al. Roles of Wnt pathway genes wls, wnt9a, wnt5b, frzb and gpc4 in regulating convergent-extension during zebrafish palate morphogenesis. Development 143, 2541–2547 (2016).

  49. 49.

    Djiane, A., Riou, J., Umbhauer, M., Boucaut, J. & Shi, D. Role of frizzled 7 in the regulation of convergent extension movements during gastrulation in Xenopus laevis. Development 127, 3091–3100 (2000).

  50. 50.

    Petridou, N. I., Grigolon, S., Salbreux, G., Hannezo, E. & Heisenberg, C. P. Fluidization-mediated tissue spreading by mitotic cell rounding and non-canonical Wnt signalling. Nat. Cell Biol. 21, 169–178 (2019).

  51. 51.

    Capek, D. et al. Light-activated Frizzled7 reveals a permissive role of non-canonical Wnt signaling in mesendoderm cell migration. eLife 8, e42093 (2019).

  52. 52.

    Ferrari, M. E. et al. Wnt7b signalling through Frizzled-7 receptor promotes dendrite development by coactivating CaMKII and JNK. J. Cell Sci. 131, jcs216101 (2018).

  53. 53.

    Sepich, D. S., Usmani, M., Pawlicki, S. & Solnica-Krezel, L. Wnt/PCP signaling controls intracellular position of MTOCs during gastrulation convergence and extension movements. Development 138, 543–552 (2011).

  54. 54.

    Montcouquiol, M. et al. Identification of Vangl2 and Scrb1 as planar polarity genes in mammals. Nature 423, 173–177 (2003).

  55. 55.

    Montcouquiol, M. et al. Asymmetric localization of Vangl2 and Fz3 indicate novel mechanisms for planar cell polarity in mammals. J. Neurosci. 26, 5265–5275 (2006).

  56. 56.

    Stoller, M. L., Roman, O. Jr. & Deans, M. R. Domineering non-autonomy in Vangl1;Vangl2 double mutants demonstrates intercellular PCP signaling in the vertebrate inner ear. Dev. Biol. 437, 17–26 (2018).

  57. 57.

    Yin, H., Copley, C. O., Goodrich, L. V. & Deans, M. R. Comparison of phenotypes between different vangl2 mutants demonstrates dominant effects of the Looptail mutation during hair cell development. PLoS ONE 7, e31988 (2012).

  58. 58.

    Hammerschmidt, M. et al. Mutations affecting morphogenesis during gastrulation and tail formation in the zebrafish, Danio rerio. Development 123, 143–151 (1996).

  59. 59.

    Jessen, J. R. et al. Zebrafish trilobite identifies new roles for Strabismus in gastrulation and neuronal movements. Nat. Cell Biol. 4, 610–615 (2002).

  60. 60.

    Lush, M. E. & Piotrowski, T. Sensory hair cell regeneration in the zebrafish lateral line. Dev. Dyn. 243, 1187–1202 (2014).

  61. 61.

    Romero-Carvajal, A. et al. Regeneration of sensory hair cells requires localized interactions between the Notch and Wnt Pathways. Dev. Cell 34, 267–282 (2015).

  62. 62.

    Harris, J. A. et al. Neomycin-induced hair cell death and rapid regeneration in the lateral line of zebrafish (Danio rerio). J. Assoc. Res. Otolaryngol. 4, 219–234 (2003).

  63. 63.

    Itoh, M. & Chitnis, A. B. Expression of proneural and neurogenic genes in the zebrafish lateral line primordium correlates with selection of hair cell fate in neuromasts. Mech. Dev. 102, 263–266 (2001).

  64. 64.

    Jiang, L., Romero-Carvajal, A., Haug, J. S., Seidel, C. W. & Piotrowski, T. Gene-expression analysis of hair cell regeneration in the zebrafish lateral line. Proc. Natl Acad. Sci. USA 111, E1383–E1392 (2014).

  65. 65.

    Jing, L., Lefebvre, J. L., Gordon, L. R. & Granato, M. Wnt signals organize synaptic prepattern and axon guidance through the zebrafish unplugged/MuSK receptor. Neuron 61, 721–733 (2009).

  66. 66.

    Lush, M. E. et al. scRNA-Seq reveals distinct stem cell populations that drive hair cell regeneration after loss of Fgf and Notch signaling. eLife 8, e44431 (2019).

  67. 67.

    Jones, C. et al. Ankrd6 is a mammalian functional homolog of Drosophila planar cell polarity gene diego and regulates coordinated cellular orientation in the mouse inner ear. Dev. Biol. 395, 62–72 (2014).

  68. 68.

    Deans, M. R. et al. Asymmetric distribution of prickle-like 2 reveals an early underlying polarization of vestibular sensory epithelia in the inner ear. J. Neurosci. 27, 3139–3147 (2007).

  69. 69.

    Wang, J. et al. Regulation of polarized extension and planar cell polarity in the cochlea by the vertebrate PCP pathway. Nat. Genet. 37, 980–985 (2005).

  70. 70.

    Duncan, J. S. et al. Celsr1 coordinates the planar polarity of vestibular hair cells during inner ear development. Dev. Biol. 423, 126–137 (2017).

  71. 71.

    Sienknecht, U. J., Anderson, B. K., Parodi, R. M., Fantetti, K. N. & Fekete, D. M. Non-cell-autonomous planar cell polarity propagation in the auditory sensory epithelium of vertebrates. Dev. Biol. 352, 27–39 (2011).

  72. 72.

    Jiang, T., Kindt, K. & Wu, D. K. Transcription factor Emx2 controls stereociliary bundle orientation of sensory hair cells. eLife 6, e23661 (2017).

  73. 73.

    Sapede, D., Gompel, N., Dambly-Chaudiere, C. & Ghysen, A. Cell migration in the postembryonic development of the fish lateral line. Development 129, 605–615 (2002).

  74. 74.

    Aw, W. Y., Heck, B. W., Joyce, B. & Devenport, D. Transient tissue-scale deformation coordinates alignment of planar cell polarity junctions in the mammalian skin. Curr. Biol. 26, 2090–2100 (2016).

  75. 75.

    Chien, Y. H., Srinivasan, S., Keller, R. & Kintner, C. Mechanical strain determines cilia length, motility, and planar position in the left-right organizer. Dev. Cell 45, 316–330 e314 (2018).

  76. 76.

    Chien, Y. H., Keller, R., Kintner, C. & Shook, D. R. Mechanical strain determines the axis of planar polarity in ciliated epithelia. Curr. Biol. 25, 2774–2784 (2015).

  77. 77.

    Olguin, P., Glavic, A. & Mlodzik, M. Intertissue mechanical stress affects Frizzled-mediated planar cell polarity in the Drosophila notum epidermis. Curr. Biol. 21, 236–242 (2011).

  78. 78.

    Aigouy, B. et al. Cell flow reorients the axis of planar polarity in the wing epithelium of Drosophila. Cell 142, 773–786 (2010).

  79. 79.

    Escobedo, N. et al. Syndecan 4 interacts genetically with Vangl2 to regulate neural tube closure and planar cell polarity. Development 140, 3008–3017 (2013).

  80. 80.

    Wang, Y., Guo, N. & Nathans, J. 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 (2006).

  81. 81.

    Gurdon, J. B., Mitchell, A. & Mahony, D. Direct and continuous assessment by cells of their position in a morphogen gradient. Nature 376, 520–521 (1995).

  82. 82.

    Barone, V. et al. An effective feedback loop between cell-cell contact duration and morphogen signaling determines cell fate. Dev. Cell 43, 198–211 e112 (2017).

  83. 83.

    Devenport, D., Oristian, D., Heller, E. & Fuchs, E. Mitotic internalization of planar cell polarity proteins preserves tissue polarity. Nat. Cell Biol. 13, 893–902 (2011).

  84. 84.

    Thery, M. et al. The extracellular matrix guides the orientation of the cell division axis. Nat. Cell Biol. 7, 947–953 (2005).

  85. 85.

    Bosveld, F. et al. Epithelial tricellular junctions act as interphase cell shape sensors to orient mitosis. Nature 530, 495–498 (2016).

  86. 86.

    Choe, C. P. et al. Wnt-dependent epithelial transitions drive pharyngeal pouch formation. Dev. Cell 24, 296–309 (2013).

  87. 87.

    Dzamba, B. J., Jakab, K. R., Marsden, M., Schwartz, M. A. & DeSimone, D. W. Cadherin adhesion, tissue tension, and noncanonical Wnt signaling regulate fibronectin matrix organization. Dev. Cell 16, 421–432 (2009).

  88. 88.

    Cavodeassi, F. et al. Early stages of zebrafish eye formation require the coordinated activity of Wnt11, Fz5, and the Wnt/beta-catenin pathway. Neuron 47, 43–56 (2005).

  89. 89.

    Matis, M. & Axelrod, J. D. Regulation of PCP by the fat signaling pathway. Genes Dev. 27, 2207–2220 (2013).

  90. 90.

    Thomas, C. & Strutt, D. The roles of the cadherins fat and dachsous in planar polarity specification in Drosophila. Dev. Dyn. 241, 27–39 (2012).

  91. 91.

    Casal, J., Lawrence, P. A. & Struhl, G. Two separate molecular systems, Dachsous/Fat and Starry night/Frizzled, act independently to confer planar cell polarity. Development 133, 4561–4572 (2006).

  92. 92.

    Casal, J., Ibanez-Jimenez, B. & Lawrence, P. A. Planar cell polarity: the prickle gene acts independently on both the Ds/Ft and the Stan/Fz systems. Development 145, dev168112 (2018).

  93. 93.

    Mangione, F. & Martin-Blanco, E. The dachsous/fat/four-jointed pathway directs the uniform axial orientation of epithelial cells in the Drosophila abdomen. Cell Rep. 25, 2836–2850 e2834 (2018).

  94. 94.

    Stemple, D. L. et al. Mutations affecting development of the notochord in zebrafish. Development 123, 117–128 (1996).

  95. 95.

    Banerjee, S. et al. A novel role for MuSK and non-canonical Wnt signaling during segmental neural crest cell migration. Development 138, 3287–3296 (2011).

  96. 96.

    Heisenberg, C. P. et al. Genes involved in forebrain development in the zebrafish, Danio rerio. Development 123, 191–203 (1996).

  97. 97.

    Quesada-Hernandez, E. et al. Stereotypical cell division orientation controls neural rod midline formation in zebrafish. Curr. Biol. 20, 1966–1972 (2010).

  98. 98.

    Wada, H. et al. Dual roles of zygotic and maternal Scribble1 in neural migration and convergent extension movements in zebrafish embryos. Development 132, 2273–2285 (2005).

  99. 99.

    Haas, P. & Gilmour, D. Chemokine signaling mediates self-organizing tissue migration in the zebrafish lateral line. Dev. Cell 10, 673–680 (2006).

  100. 100.

    Kindt, K. S., Finch, G. & Nicolson, T. Kinocilia mediate mechanosensitivity in developing zebrafish hair cells. Dev. Cell 23, 329–341 (2012).

  101. 101.

    Kozlovskaja-Gumbriene, A. et al. Proliferation-independent regulation of organ size by Fgf/Notch signaling. eLife 6, e21049 (2017).

  102. 102.

    Parinov, S., Kondrichin, I., Korzh, V. & Emelyanov, A. Tol2 transposon-mediated enhancer trap to identify developmentally regulated zebrafish genes in vivo. Dev. Dyn. 231, 449–459 (2004).

  103. 103.

    Lush, M. E. & Piotrowski, T. ErbB expressing Schwann cells control lateral line progenitor cells via non-cell-autonomous regulation of Wnt/beta-catenin. eLife 3, e01832 (2014).

  104. 104.

    Ma, E. Y., Rubel, E. W. & Raible, D. W. Notch signaling regulates the extent of hair cell regeneration in the zebrafish lateral line. J. Neurosci. 28, 2261–2273 (2008).

  105. 105.

    Kopinke, D., Sasine, J., Swift, J., Stephens, W. Z. & Piotrowski, T. Retinoic acid is required for endodermal pouch morphogenesis and not for pharyngeal endoderm specification. Dev. Dyn. 235, 2695–2709 (2006).

  106. 106.

    Venero Galanternik, M., Kramer, K. L. & Piotrowski, T. Heparan sulfate proteoglycans regulate Fgf signaling and cell polarity during collective cell migration. Cell Rep. 10, 414–428 (2015).

  107. 107.

    Nikaido, M., Law, E. W. & Kelsh, R. N. A systematic survey of expression and function of zebrafish frizzled genes. PLoS One 8, e54833 (2013).

  108. 108.

    Schindelin, J. et al. Fiji: an open-source platform for biological-image analysis. Nat. Methods 9, 676–682 (2012).

  109. 109.

    Butler, M. T. & Wallingford, J. B. Spatial and temporal analysis of PCP protein dynamics during neural tube closure. eLife 7, e36456 (2018).

  110. 110.

    Kwan, K. M. et al. The Tol2kit: a multisite gateway-based construction kit for Tol2 transposon transgenesis constructs. Dev. Dyn. 236, 3088–3099 (2007).

  111. 111.

    Smith, S. E. et al. Independence of symmetry breaking on Bem1-mediated autocatalytic activation of Cdc42. J. Cell Biol. 202, 1091–1106 (2013).

  112. 112.

    Bevington, P. R. & Robinson, D. K. Data Reduction and Error Analysis for the Physical Sciences 3rd edn (McGraw-Hill, 2003).

  113. 113.

    Klingenberg, C. P. MorphoJ: an integrated software package for geometric morphometrics. Mol. Ecol. Resour. 11, 353–357 (2011).

  114. 114.

    Moreno-Mateos, M. A. et al. CRISPRscan: designing highly efficient sgRNAs for CRISPR-Cas9 targeting in vivo. Nat. Methods 12, 982–988 (2015).

  115. 115.

    Montague, T. G., Cruz, J. M., Gagnon, J. A., Church, G. M. & Valen, E. CHOPCHOP: a CRISPR/Cas9 and TALEN web tool for genome editing. Nucleic Acids Res. 42, W401–W407 (2014).

  116. 116.

    Varshney, G. K. et al. High-throughput gene targeting and phenotyping in zebrafish using CRISPR/Cas9. Genome Res. 25, 1030–1042 (2015).

Download references


We would like to thank Drs. R. Krumlauf, M. Lush, and S. Baek for comments on the paper and the Piotrowski lab members for lively discussions. We also thank Dr. R. Duncan for the initial wnt11 (wnt11f1) in situ analysis, the Aquatics Facility of the Stowers Institute for Medical Research for their outstanding husbandry work. We grateful to T. Nicolson for sending us the myo6b:β-Actin-GFP fish, C. Walsh for the scribble mutants, D. Slusarski for the wnt5b mutants, and J. Wallingford for the Xenopus GFP-Vangl2 construct; and L. Solnica-Krezel, A. Chandrasekhar, M. Harris, R. Burdine, B. Ciruna, C.P. Heisenberg, and B. Link for reagents used in pilot studies. Many thanks also to D. Diaz for help with the bioinformatic analysis. This work was funded by an NIH award RO1 NS082567 to C.M., an NIH (NIDCD) award 1R01DC015488-01A1 to T.P and by institutional support from the Stowers Institute for Medical Research to T.P. J.N.A. is a Predoctoral Researcher at the Graduate School of the Stowers Institute for Medical Research.

Author information

J.N.A. designed the experiments, collected, analyzed, and interpreted the data, and wrote the paper; R.L.A., T.W., J.R.U., and H.L. analyzed the data; C.M. provided the wnt11 (wnt11f1)fh224 mutants; M.G.V. discovered the hair cell orientation phenotype in wnt11 (wnt11f1) mutants. T.P. designed and interpreted the experiments, and wrote the paper.

Correspondence to Tatjana Piotrowski.

Ethics declarations

Competing interests

The authors declare no competing interests.

Additional information

Peer review information: Nature Communications thanks the anonymous reviewers for their contribution to the peer review of this work. Peer reviewer reports are available.

Publisher’s note: Springer Nature remains neutral with regard to jurisdictional claims in published maps and institutional affiliations.

Supplementary information

Source data

Rights and permissions

Open Access This article is licensed under a Creative Commons Attribution 4.0 International License, which permits use, sharing, adaptation, distribution and reproduction in any medium or format, as long as you give appropriate credit to the original author(s) and the source, provide a link to the Creative Commons license, and indicate if changes were made. The images or other third party material in this article are included in the article’s Creative Commons license, unless indicated otherwise in a credit line to the material. If material is not included in the article’s Creative Commons license and your intended use is not permitted by statutory regulation or exceeds the permitted use, you will need to obtain permission directly from the copyright holder. To view a copy of this license, visit http://creativecommons.org/licenses/by/4.0/.

Reprints and Permissions

About this article

Verify currency and authenticity via CrossMark

Cite this article

Navajas Acedo, J., Voas, M.G., Alexander, R. et al. PCP and Wnt pathway components act in parallel during zebrafish mechanosensory hair cell orientation. Nat Commun 10, 3993 (2019) doi:10.1038/s41467-019-12005-y

Download citation


By submitting a comment you agree to abide by our Terms and Community Guidelines. If you find something abusive or that does not comply with our terms or guidelines please flag it as inappropriate.