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. 2009 May 13;136(12):1977–1986. doi: 10.1242/dev.030718

Myosin II regulates extension, growth and patterning in the mammalian cochlear duct

Norio Yamamoto 1, Takayuki Okano 1, Xuefei Ma 2, Robert S Adelstein 2, Matthew W Kelley 1,*
PMCID: PMC2685721  PMID: 19439495

Summary

The sensory epithelium of the mammalian cochlea comprises mechanosensory hair cells that are arranged into four ordered rows extending along the length of the cochlear spiral. The factors that regulate the alignment of these rows are unknown. Results presented here demonstrate that cellular patterning within the cochlea, including the formation of ordered rows of hair cells, arises through morphological remodeling that is consistent with the mediolateral component of convergent extension. Non-muscle myosin II is shown to be expressed in a pattern that is consistent with an active role in cellular remodeling within the cochlea, and genetic or pharmacological inhibition of myosin II results in defects in cellular patterning that are consistent with a disruption in convergence and extension. These results identify the first molecule, myosin II, which directly regulates cellular patterning and alignment within the cochlear sensory epithelium. Our results also provide insights into the cellular mechanisms that are required for the formation of highly ordered cellular patterns.

Keywords: Hair cell, Organ of Corti, Inner ear, Pillar cell, Mouse

INTRODUCTION

In mammals sounds are perceived by the organ of Corti (OC), a sensory epithelium that extends along the basal-to-apical axis of the cochlear spiral. The OC comprises highly ordered rows of mechanosensory hair cells and non-sensory supporting cells. The evolution of an elongated cochlea and the unique morphology of the OC represent key steps in the evolution of the ability to perceive and discriminate a wide range of auditory frequencies (von Bekesy, 1949). The mechanisms that regulate elongation of the duct and/or cellular patterning within the OC are largely unknown. However, it has recently been suggested that convergence and extension, mediated at least in part through the planar cell polarity (PCP) pathway, plays a role in both cochlear elongation and cellular patterning (Chen et al., 2002; Montcouquiol et al., 2003; McKenzie et al., 2004; Wang et al., 2005; Qian et al., 2007). Convergent extension (CE) refers to a morphogenetic process in which the three-dimensional distribution of a population of cells extends along one axis while simultaneously narrowing along a perpendicular axis (Keller et al., 2000; Keller, 2002). In some cases, CE can be preceded by a period of radial intercalation in which cells extend as a result of thinning along an axis oriented perpendicular to the axes of subsequent CE (Keller, 2000; Keller et al., 2002). CE has been observed during amphibian gastrulation (Keller, 1986) and neurulation (Jacobson and Gordon, 1976) and more recently in Drosophila germband extension (Irvine and Weischaus, 1994).

Non-muscle myosin 2 (NM II) is a hexameric protein composed of two dimeric heavy chains (NMHCs), a pair of regulatory light chains (RLCs) and a pair of essential light chains. Phosphorylation of the RLCs by a number of kinases, principally myosin light chain kinase (Kamm and Stull, 1985) and RHO-associated protein kinase (ROCK) (Amano et al., 1996; Conti and Adelstein, 2008), regulates self-assembly and ATPase activity (Conti and Adelstein, 2008). Recently, myosin II has been shown to play a significant role in CE in both Drosophila and vertebrates (Sellers, 2000; Bertet et al., 2004; Conti and Adelstein, 2008; Skoglund et al., 2008). The specific effects of NM II during CE are still poorly understood but can include junctional remodeling and changes in cell shape (Conti and Adelstein, 2008).

In humans and mice three genes encode NMHC II, MYH9, MYH10 and MYH14 (Golomb et al., 2004). Although a role for NM II in cochlear development has not been reported, both syndromic and non-syndromic hearing loss results from mutations in MYH genes, including R702H, R702C and R705H mutations in MYH9 (Lalwani et al., 2000; Heath et al., 2001) and S7X, S120L, G376C and R726S mutations in MYH14 (Donaudy et al., 2004; Yang et al., 2005). The physiological basis for the auditory defect in these individuals has not been determined, but is believed to be sensorineural in nature (Chen et al., 1995; Lalwani et al., 1997). Based on these results, it seemed likely that myosin II could play an important role in cellular patterning and/or extension of the OC during embryonic development.

MATERIALS AND METHODS

Animals

ICR mice were purchased from Charles River Laboratories. Myh9, Myh10 and Myh14 null and Myh10DN mice were described previously (Tullio et al., 1997; Conti et al., 2004; Ma et al., 2004). To restrict expression of Myh10DN to the developing ear, the Foxg1Cre line (Hebert et al., 2000) was used to remove the neomycin cassette in the otocyst, forebrain and retina. Resulting embryos survived until E16.5 and were obtained in expected ratios. All animals were maintained based on the standards outlined in the National Institutes of Health Guide for the Care and Use of Laboratory Animals.

Determination of changes in cochlear length and cellular patterning

Cochleae were dissected from embryos at specific developmental time points, the developing cochlear epithelium was exposed and cell boundaries and prosensory cells were labeled with phalloidin and anti-p27Kip1 (CDKN1B - Mouse Genome Informatics) as previously described (McKenzie et al., 2004). Changes in length and width of the prosensory domain were determined as previously described (McKenzie et al., 2004). To determine changes in individual cell shape, 150 μm of cochlear sensory epithelia located at the 50% position along the basal-to-apical axis of the cochlea length was imaged. ImageJ (http://rsb.info.nih.gov/ij/) and Metamorph (Universal Imaging) software packages were used to determine the length, width and area of each cell within the region. A minimum of three separate cochleae from different litters were analyzed for each time point. Changes in the number of specific cell types were determined by labeling cell boundaries with phalloidin and labeling cells with specific markers such as anti-myosin 6 for hair cells and anti-p75NTR (NGFR - Mouse Genome Informatics) for pillar cells.

Reverse transcriptase polymerase chain reaction

Epithelia from five E13.5 or E16.5 cochleae were isolated by treating with thermolysin (Montcouquiol and Kelley, 2003) and total RNA was extracted. cDNA was synthesized using the ABI cDNA Synthesis Kit (Applied Biosystems, Foster City, CA, USA). Sequences for primer sets for Myh9, Myh10 and Myh14 are available upon request.

Quantitative RT-PCR

Total RNA was prepared as described above. For experiments using Myh10 null mice, total RNA was extracted from two cochlear epithelia for each genotype. cDNA was mixed with Power SYBR Green PCR Master Mix (Applied Biosystems) and subjected to real-time PCR quantification using an ABI PRISM 7000 Sequence Detection System (Applied Biosystems). All reactions were performed in triplicate. The relative amounts of mRNAs were calculated by using the standard curve method. As the invariant control, we used mouse Arbp (Rplp0 - Mouse Genome Informatics) mRNA (Yabe et al., 2003). Sequences for primer sets are available upon request.

Immunohistochemistry

For whole mounts, cochleae were prepared as described in Jacques et al. (Jacques et al. 2007). For immunohistochemical analysis of sections, cochleae were dissected, fixed in 4% paraformaldehyde, cryoprotected through a sucrose gradient, embedded in Tissue-Tek (MILES, Elkhart, Illinois, USA) and sectioned on a cryostat.

Primary antibodies were: rabbit anti-MYH9 and anti-MYH10 (1:500, polyclonal, Covance); rabbit anti-MYH14 [1:500, polyclonal (Golomb et al., 2004)]; rabbit anti-myosin 6 (1:1000, polyclonal, Proteus BioSciences); rabbit anti-p27Kip1 (1:100, polyclonal, Lab Vision); and rabbit anti-p75NTR (1:1000, polyclonal, Chemicon). Specificity of anti-MYH9, anti-MYH10 and anti-MYH14 antibodies were confirmed by western blot (see Fig. S1 in the supplementary material). Actin filaments were visualized with Alexa488-conjugated phalloidin (1:200, Invitrogen-Molecular Probes).

Primary antibodies were visualized with Alexa488- or Alexa546-conjugated secondary antibodies (Invitrogen-Molecular Probes). All fluorescent images were obtained on an LSM510 laser scanning microscope (Carl Zeiss).

Determination of changes in orientation of cell-cell boundaries

Cochleae from E14 embryos were labeled with phalloidin as described. Developing hair cells were identified based on increased accumulation of actin (McKenzie et al., 2004). Cells located within 7 μm of the medial edge of the inner hair cells were classified as within the pillar cell domain and cells located between 7 and 14 μm from the medial edge of inner hair cells were classified as within the outer hair cell region. All of the cell-cell boundaries located along at least 50 μm of the basal-to-apical axis were included for each sample and a minimum of three separate cochleae were included for each location.

Assessment of cochlear extension

Cochleae were dissected from mouse embryos at E14. Following dissection, the cochlear duct was cut at the midpoint and the basal half was established as an explant culture. Explants were maintained for 4 days in vitro. At the end of each experiment, hair cells were labeled with anti-myosin 6 and the extent of outgrowth and change in width of the sensory epithelium was determined based on the distribution of hair cells. A minimum of seven explants from multiple litters were analyzed for each control or experimental group.

Cochlear explant cultures

Cochleae were isolated as described above except the epithelium was left intact. In order to visualize the sensory epithelium, the roof of the duct was removed. Explants were maintained as described previously (Montcouquiol et al., 2003). For cultures containing just the developing cochlear epithelium, cochleae were dissected as described and the epithelium was isolated by treatment with thermolysin (Montcouquiol et al., 2003). The length and width of the sensory epithelium was determined as described for the outgrowth assay.

Inhibition of NM II function in vitro

Cochlear explants were treated with 3 or 10 μM of blebbistatin (Sigma-Aldrich) or Y27632 (EMD Chemicals), plus 0.1% DMSO as a vehicle. Control explants were treated with vehicle alone.

RESULTS

The cochlear sensory epithelium extends between E14 and E16

The sensory epithelium of the mammalian cochlea originates in the basal region of the cochlear spiral located near the oval window and continues as a narrow strip of cells to the apex located at the tip of the coil (apicobasal axis). The width of the epithelium is measured along the mediolateral axis oriented perpendicular to the apicobasal axis. At any point along the cochlea, the thickness of the epithelium spans from the basement membrane to the lumenal surface (basolumenal axis). Previous results have demonstrated that the developing sensory epithelium undergoes significant extension between E14 and E16, with E16 representing the earliest time at which the final cellular pattern of the OC can be identified (Cantos et al., 2000; McKenzie et al., 2004). To confirm these results, prosensory cells were identified based on expression of p27Kip1 (Chen and Segil, 1999) and the overall dimensions of the prosensory domain were determined at E14 and E16. Results indicated changes in the length and width of the prosensory domain (Fig. 1A-C) that are consistent with convergence and extension as suggested by Chen and Segil (Chen and Segil, 1999) and McKenzie et al. (McKenzie et al., 2004).

Fig. 1.

Fig. 1.

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Convergence and extension of the cochlear prosensory domain. (A,B) Whole mounts of the cochlea at E14 (A) and E16 (B). The prosensory domain is marked by expression of p27Kip1 (arrows). Note the extension and narrowing of the prosensory domain (arrows) that occurs between E14 and E16. (C) Comparison of changes in length, width, length/width ratio and surface area of the sensory epithelium between E14 and E16. There is a significant increase in length, a significant decrease in width and a significant increase in overall area. (D,E) Phalloidin labeling (green) of cell-cell boundaries in the cochlear duct. The prosensory domain is illustrated in violet. Arrows in D indicate orientation of length and width axes. The lower aspect of each panel illustrates outlines for individual cells within the prosensory domain. (F) Comparison of changes in length, width, length/width ratio, surface area, and cell density per unit length and across the width of the sensory epithelium between E14 and E16. The decrease in density of cells along the width of the epithelium is consistent with ongoing convergence. Scale bars: 200 μm in A,B; 10 μm in E (same magnification in D). *P<0.005, **P<0.05, ***P<0.0001.

Changes in cell shape correlate with extension of the cochlear duct

To determine changes in individual cell shapes during the E14 to E16 period of extension, the lumenal dimensions of each prosensory cell were identified by labeling cortical actin with phalloidin (Fig. 1D,E). Average lumenal morphologies for over 500 prosensory cells were determined in a region of the cochlear duct located at the midpoint along the apicobasal axis of the cochlea. At E14, the majority of prosensory cells have rounded lumenal profiles with a length (measured along the apicobasal axis) to width (measured along the mediolateral axis) ratio of ∼1.4 and an average lumenal surface area of ∼5.0 μm2 (Fig. 1F). By E16, lumenal surfaces have significantly increased both in length and in width leading to a doubling in the average surface area. In addition, there is a small but significant increase in the length/width ratio, indicating a disproportionate lengthening of each cell. The observation that individual cell width actually increases between E14 and E16, while the overall width of the sensory epithelium decreases, suggests that the data in Fig. 1 probably underestimate the amount of convergence that occurs. Finally, the increase in the lumenal surface area of each cell, along with the decrease in the width of the sensory epithelium, results in a significant decrease in the density of prosensory cells along both the apicobasal and proximodistal axes (Fig. 1F).

Myh9, Myh10 and Myh14 are expressed in the cochlear epithelium

The data presented above suggested a role for CE and growth during the development of the OC. To determine whether NM II plays a role in these events, the expression of mRNA for all three NMHCs within the developing sensory epithelium was determined. Results of RT-PCR analysis indicated that, in addition to other tissues, all three MYH genes are expressed in the cochlear epithelium at both E13.5 and E16.5 (see Fig. S2 in the supplementary material). None of the reported splice variants of Myh10 (Itoh and Adelstein, 1995) was observed in the cochlea, but all of the splice variants for Myh14 (Golomb et al., 2004) were present.

Next, developmental changes in the level of expression of each MYH gene within the cochlea were determined by quantitative RT-PCR (see Fig. S2 in the supplementary material). Expression of Myh9 steadily decreased between E12.5 and E16.5. Expression of Myh10 also decreased during the same time period, but the relative level of decrease was less than for Myh9. By contrast, expression of Myh14 increased nearly sixfold between E12.5 and E16.5. This result is consistent with previous results showing that Myh14 is more abundant in adult tissues (Golomb et al., 2004).

MYH10 and MYH14 are asymmetrically distributed in developing cochlear sensory epithelial cells

To determine the cellular and subcellular distribution of each of the MYH proteins within the developing cochlea, immunohistochemical localization was carried out in both whole mounts and cryostat sections at E13.5 and E16. MYH9 immunoreactivity is limited and diffuse throughout the cochlea at both time periods (see Fig. S3 in the supplementary material) although MYH9 is observed in other tissues, such as the neural tube. By contrast, at E13.5 MYH10 and MYH14 are distributed uniformly around the lumenal surface in all cells of the developing sensory epithelium (data not shown). To examine the change in distribution of MYH10 and MYH14 during the period of cochlear extension, the localization of both proteins was studied in E16 cochleae. The sensory epithelium of the cochlea develops in a gradient that extends from base to apex. At E16, the sensory epithelium at the base of the cochlea is comparatively mature with a recognizable pattern of hair cells and supporting cells. By contrast, the apex of the cochlea at E16 appears undifferentiated with no obvious cellular patterning. Therefore, changes in developmental distribution of MYH proteins could be examined in a single cochlea. In the undifferentiated apex of the cochlea, MYH10 distribution is largely homogenous, with a slight increase in expression that forms a faint line oriented along the apicobasal axis and located near the medial boundary of the sensory epithelium (Fig. 2A). In the mid-apical and middle regions of the cochlea, two lines of MYH10 are obvious, one (continuous with the faint line observed in the apical region) that correlates with the boundary between inner hair cells and inner pillar cells (IPCs) and a second one located at the apparent lateral boundary of the sensory epithelium (see Fig. 2B for explanation of cellular patterning in the OC). In the mid-basal region, a third line of MYH10, located between the IPCs and the first row of outer hair cells, is apparent. In addition, the distance between the first two lines of MYH10 is decreased (from an average of 10.06 μm to 7.56 μm), consistent with convergence of the sensory epithelium. Finally, in the basal region, the three lines of MYH10 persist and the distance between the first and second lines is decreased even further. Moreover, additional lines of MYH10, also oriented along the axis of extension (apicobasal axis), are present between the rows of developing outer hair cells.

Fig. 2.

Fig. 2.

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Distribution of MYH10 and MYH14 along the basal-to-apical axis of the cochlea at E16.5. (A) In the apical region, MYH10 distribution (red) is largely uniform at all cell boundaries, with the exception of a faint line of increased intensity (arrow) near the medial edge of the sensory epithelium (see Fig. 2B for diagram of cellular pattern in mature OC). The position of developing inner hair cells (IHC) is indicated for orientation. In the mid-apical and middle regions, two lines are present, a line located between IHCs and IPCs (arrow) that is continuous with the line in the apical region, and a second line located at the extreme lateral edge of the OC (arrowhead). In the mid-basal region, a third line located at the boundary between IPCs and OHCs is also present (angled arrow). In the basal region shorter lines are also present between each row of OHCs. (B) Diagram illustrating the cellular pattern in the OC. (C) Distribution of MYH14 (red). In the mid-apical region, MYH14 is uniformly distributed with slightly brighter labeling at the boundary between IHCs and IPCs (arrow). In more mature regions, MYH14 is prominent at all boundaries of PCs, IHCs and IPhs but labeling is considerably reduced in the OHC region. (D,E) Cross-sections through the cochlear duct at E16.5 illustrating the distribution of MYH10 (D) and MYH14 (E). Bracket indicates the sensory epithelium in D and Kolliker's organ in E. Asterisk in E indicates the sensory epithelium. IHC, Inner hair cell; IPh, Inner phalangeal cell; IPC, Inner pillar cell; OPC, Outer pillar cell; OHC, Outer hair cell; SC, Supporting cell. Scale bars: 10 μm in A,C; 15 μm in E (same magnification in D).

In contrast to MYH10, in E16 cochleae MYH14 is predominantly localized to the developing IPCs, inner hair cells and inner phalangeal cells. In the apical and mid-apical regions, MYH14 is uniformly distributed throughout the sensory epithelium, however, more prominent labeling is present on the medial edges of developing IPCs, resulting in a line oriented along the axis of extension (Fig. 2C). In the middle and mid-basal regions, MYH14 labeling is decreased in the outer hair cell region, but becomes more prominent in the IPC and inner hair cell regions. Finally, in the mature basal region, MYH14 is prominently distributed in IPCs and inner phalangeal cells and might also be expressed in inner hair cells. By contrast, labeling is almost completely absent in the outer hair cell region. Specificity of each antibody was confirmed by western blot and no primary control (see Figs S1 and S3 in the supplementary material).

Cell shape changes in the sensory epithelium are consistent with convergence and extension

The marked distribution of MYH10 and MYH14 in developing IPCs suggested that these cells might play an important role in cochlear CE. Previous results suggest that changes in cell shape, and in particular increased length along the axis of elongation, provide at least some of the driving forces for CE (Bertet et al., 2004). The initial analysis of changes in cell shape within the developing sensory epithelium between E14 and E16 had indicated only minor changes in the overall length/width ratio for all cells within the sensory epithelium (Fig. 1F). However, during this analysis, a subset of cells with elongated axes oriented parallel to the direction of elongation were observed adjacent to developing inner hair cells, a position consistent with the location of developing IPCs (Fig. 3A). To determine whether these elongated cells might indicate a region of ongoing extension, the total length of cell-cell contacts oriented parallel, perpendicular or intermediate to the axis of elongation was determined (Fig. 3B,C). For comparison, cells located in different regions of the epithelium, or in the same region but at an earlier time point, were also analyzed. Results indicated that cells located adjacent to developing inner hair cells undergo a significant change in cell shape that includes lengthening along the apicobasal axis of the cochlea and shortening along the medial-to-lateral axis. Cells located slightly farther from the developing inner hair cell region, but still within the developing sensory epithelium, showed similar but less pronounced cell shape changes, whereas cells located medial to the sensory epithelium did not change shape.

Fig. 3.

Fig. 3.

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Developing pillar cells undergo cell shape changes that are consistent with CE. (A) Middle region of the cochlea at E14. Cells located in the developing pillar cell (PC) and outer hair cell (OHC) domains, adjacent to developing inner hair cells (arrows), appear flattened. (B) Outlines of individual cells (colored for clarity) in three different regions of the cochlea. See A for orientation. Cells located adjacent to developing inner hair cells (asterisks) are flattened in comparison with cells located medial or lateral to the developing sensory epithelium. (C) Cell boundaries were classified as either parallel (0° to 30°, blue), perpendicular (61° to 90°, green) or intermediate (31° to 60°, red) to the axis of extension (black two-headed arrow). (D) Comparison of the ratios of different orientations of cell boundaries, as described in C, within the sensory epithelium between E13 and E14. Parallel boundaries are increased at the expense of intermediate and perpendicular boundaries. (E) Comparison of cell boundaries as in D, in different regions within the same cochlea at E14. A significantly greater proportion of cell-cell boundaries are oriented parallel to the axis of extension in the pillar cell region as compared with a non-sensory region. The outer hair cell region shows a similar distribution of boundary orientations, but values were not significantly different from the non-sensory region. Data for E14 pillar cell region are the same as for E14 in D. Scale bar: 10 μm. *P<0.01.

Expression of dominant negative Myh10 inhibits extension and disrupts cellular patterning in the cochlea

To determine whether myosin II plays a role in cochlear extension, mice with targeted mutations in each of the MYH genes were analyzed. Deletion of Myh9 results in embryonic lethality at E7.5 (Conti et al., 2004). Since this is well before the onset of cochlear development, no analysis of cochlear extension was possible in Myh9 mutants. By contrast, Myh10 null mice survive until E15 (Tullio et al., 1997) and Myh14 null mice are viable. However, no defects were observed in the length or overall morphology of the cochleae in either mutant (data not shown). Considering that all three MYH proteins are expressed in the embryonic cochlea, functional or genetic compensation, as has been reported in the embryonic heart (Tullio et al., 1997), seemed possible. Although quantitative PCR for Myh14 in Myh10 mutants indicated no change in the level of Myh14 expression (data not shown), compensation at post-transcriptional levels cannot be ruled out.

Therefore, to examine the effects of reduced MYH function, we analyzed cochleae from mice carrying a putative dominant negative mutation (R709C) in Myh10 (Ma et al., 2004). Previous studies have demonstrated that mutations in the conserved R709 residue compromise actin-activated MgATPase activity and in vitro motility, as well as inhibiting the activity of wild-type MYHs (Kim et al., 2005). Activation of the Myh10R709C mutation (referred to as Myh10DN) in the inner ear was accomplished using Foxg1Cre (see Materials and methods for details). The resulting Myh10DN/DN;Foxg1Cre/+ mice survived until E16.5 and were obtained at expected mendelian ratios.

To determine whether myosin II regulates extension, the length and width of the prosensory domain was determined in experimental (Myh10DN/DN;Foxg1Cre/+) and control (Myh10+/+;Foxg1Cre/+) cochleae at E16 (Fig. 4A-D). Results indicated a significantly shorter prosensory domain in the cochleae of experimental versus control embryos (Fig. 4E). A corresponding increase in the width of the prosensory domain was not observed in experimental cochleae, except in the apex (Fig. 4B). However, the average lumenal surface of prosensory cells was significantly reduced (Fig. 4E), whereas the density of cells along the basal-to-apical axis was significantly increased (Fig. 4E). These results suggest that expression of Myh10DN inhibits both convergence and extension, as observed by the increase in cell density, and cell growth, based on the decreased lumenal surface areas of cells within the prosensory region.

Fig. 4.

Fig. 4.

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Myh10DN inhibits CE and disrupts cellular patterning. (A,B) Whole mounts of E16 cochleae from a control (A) and an Myh10DN mutant (B). The prosensory domain is marked by p27Kip1. Note that the sensory epithelium appears shorter along the length and wider in the apex in the mutant. (C) Upper panel illustrates individual cell boundaries within the developing sensory epithelium (violet) in the middle region of the cochlea from a control embryo at E16. Lower panel illustrates pattern of hair cells (red). (D) Similar view as in C, except from an Myh10DN mutant. Cellular pattern is disrupted, average cell size appears smaller and expression of myosin 6 is decreased as compared with the control, which could be a result of direct downregulation. Also, alignment of hair cells is disrupted. (E) Quantification of changes in morphometric parameters. The length of the sensory epithelium is significantly decreased in Myh10DN cochleae but the width is unchanged as a result of a significant increase in cell density. (F-K) The sensory epithelium in control and Myh10DN cochleae. (F) Fluorescent image of the sensory epithelium in the middle region of the cochlea from an E16 control embryo. Cell borders are labeled with phalloidin (green) and hair cells are marked with anti-myosin 6 (red). (G) Line drawing derived from the image in F, with cell types marked as follows: hair cells, blue; supporting cells, yellow; pillar cells, pink. (H) Comparable image to F, but from an Myh10DN cochlea. Note the decreased cell size and disrupted organization. (I) Line drawing as in G. Rather than a single row, multiple rows of pillar cells (pink) are present. (J,K) Sensory epithelium in the middle region of the cochlea from an E16 control (J) and an Myh10DN (K) embryo. Inner pillar cells are labeled with anti-p75NTR (red). A single row of inner pillar cells (arrow) is present in the control. Three additional p75NTR-positive cells are present adjacent to the developing inner pillar cell row (just above the arrow). By contrast, two rows of inner pillar cells are present in the mutant (arrows) and additional anti-p75NTR-positive cells (arrowheads) are located in the outer hair cell domain. Insets: line drawings of the inner pillar cells in J and K (not to scale). Scale bars: 200 μm in A,C; 10 μm in B,D,F (same magnification in J,H,K). *P<0.01, **P<0.02, ***P<0.05.

The strong expression of MYH10 and MYH14 in IPCs suggested that the development of these cells might be specifically regulated by myosin II. To examine this possibility, the IPC region was visualized at the midpoint of the cochlea in control and Myh10DN experimental cochleae. Results indicated an increase in the number of cells within the IPC region in cochleae from experimental embryos (76.5 IPCs/100 μm in Myh10DN experimental versus 32.2 IPCs/100 μm in control, P=0.004; Fig. 4F-I). In addition, all of these cells retained a rounded morphology rather than a cuboidal or elongated shape. The identity of these cells as IPCs was confirmed by labeling with the IPC marker p75NTR (Fig. 4J,K). However, a similar analysis in the more mature basal region of the cochlea in both control and experimental cochleae indicated a progressive improvement in overall cellular patterning in the Myh10DN cochleae, suggesting a delay, rather than a complete disruption, in cellular patterning (data not shown). These results suggest that the Myh10DN allele does not completely inhibit the activity of myosin II.

Finally, to determine whether a disruption in radial intercalation could contribute to the patterning defects observed in Myh10DN cochleae, the thickness of the epithelium along the basolumenal axis was examined in cross sections from wild type and Myh10DN mutants. No change in epithelial thickness was observed (see Fig. S4 in the supplementary material), suggesting that radial intercalation was not affected in Myh10DN mutants.

Pharmacological inhibition of myosin II function inhibits extension of the sensory epithelium

As the extent of the dominant negative activity of Myh10DN has not been determined, we sought to further examine the effects of inhibition of myosin II in cochlear explant cultures using three different myosin II antagonists: blebbistatin, which selectively inhibits myosin II (Straight et al., 2003; Limouze et al., 2004; Kovacs et al., 2004); the RHO-associated protein kinase (ROCK) inhibitor, Y27632 (Kimura et al., 1996; Amano et al., 1996; Uehata et al., 1997); and ML7, an inhibitor of myosin light chain kinase (Wadgaonkar et al., 2005; Bessard et al., 2006). Effects of inhibition of myosin II on cochlear extension were quantified using a previously described in vitro outgrowth assay (Wang et al., 2005) (see Materials and methods for details). In control explants, the average extension of the sensory epithelium was ∼600 μm (Fig. 5A,B,G). By contrast, treatment with blebbistatin (Fig. 5C) or Y27632 (Fig. 5D) resulted in a significant inhibition of extension by comparison with no treatment or exposure to either N-benzyl-p-toluene sulfonamide (BTS), a specific inhibitor of skeletal muscle myosin (Cheung et al., 2002), or to ML7 (Fig. 5G and data not shown). At 10 μM of blebbistatin, the highest tolerable concentration, extension of the sensory epithelium was reduced to ∼150 μm, a 75% reduction from control sensory epithelium (Fig. 5G). In contrast with extension, the width of the sensory epithelium was only significantly increased in explants treated with the highest dose (10 μM) of blebbistatin (Fig. 5H). These results are consistent with the phenotypic changes observed in Myh10DN mutant cochleae. Disruptions in cellular patterning in blebbistatin-treated explants appeared comparable with, but more severe than, the disruptions observed in Myh10DN mutants (Fig. 5E,F). In addition to multiple rows of IPCs, outer hair cells and, to a lesser extent, inner hair cells also failed to align into the characteristic one row of inner hair cells and three rows of outer hair cells (Fig. 5E,F). In addition, individual cell length, width and overall area showed decreases that were comparable to those observed in Myh10DN mutants (Fig. 5I). Finally, to confirm that treatment with blebbistatin did not lead to a disruption of junctional complexes, expression of the tight junction protein ZO1 (TJP1 - Mouse Genome Informatics) was examined in control and blebbistatin-treated explants (Fig. 5J,K). Although patterning defects are evident in response to blebbistatin, ZO1 is still restricted to the lumenal boundaries of each cell, suggesting that the epithelial integrity is intact.

Fig. 5.

Fig. 5.

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Inhibition of myosin II activity disrupts cochlear CE. (A) Outgrowth of the sensory epithelium was assayed by cutting the intact cochlear duct at its midpoint and then maintaining the basal piece in vitro. Over the subsequent 72-96 hours the sensory epithelium extended outwards from the cut end of the explant. (B) Control explant established as described in A. The site of the initial cut is marked in white. The sensory epithelium (hair cells marked in red) extends from the initial cut site. (C) Explant established as in B, but treated with 10 μM of the myosin II inhibitor blebbistatin beginning at E14. The sensory epithelium is noticeably shorter and wider. (D) An explant established as in B, but treated with 10 μM of the ROCK inhibitor Y27632. The phenotype of the sensory epithelium is similar to that in C. (E,F) Images of the sensory epithelium from control (E) and 10 μM blebbistatin-treated (F) explants labeled with anti-myosin 6 (red) and phalloidin (green). Additional inner pillar cells (PC) are present in blebbistatin-treated explants. Patterning in the IHCs and OHCs is also disrupted. Abbreviations as in Fig. 2. (G) Treatment with either blebbistatin or Y27632 results in a significant and dose-dependent decrease in extension of the sensory epithelium. By contrast, the skeletal muscle myosin inhibitor BTS did not affect extension. (H) Treatment with 10 μM blebbistatin leads to a significant increase in the width of the sensory epithelium. However, the width of the sensory epithelium was not significantly increased in explants treated with 10 μM Y27632. (I) Blebbistatin treatment leads to changes in cell shape that are consistent with changes in Myh10DN mutants. (J,K) Surface (upper panel) and cross-section (lower panel) views of control (J) and blebbistatin-treated (K) explants labeled with an antibody specific for the tight junction protein ZO1 (green). Tight junctions are present in explants from both conditions and are restricted to the lumenal surfaces. Scale bars: 50 μm in B (same magnification in C,D); 20 μm in E (same magnification in F,I,J). *P<0.005, **P<0.001, ***P<0.01.

Inhibition of myosin II leads to changes in inner pillar cell morphology

The analysis of changes in cell morphology had suggested that developing IPCs become more flattened during the period of extension. To determine whether changes in IPC shapes are regulated through myosin II, IPCs were specifically labeled in explants that had been treated with blebbistatin for 48 hours beginning at E14. The overall length of the sensory epithelium was shorter in blebbistatin-treated explants and the row of IPCs was disorganized (Fig. 6). In addition, the lumenal profiles of individual IPCs indicated that inhibition of myosin II resulted in cells that had failed to flatten. Quantification of the lengths and widths of individual IPCs indicated a significant decrease in the length and a significant increase in the width of IPCs in blebbistatin-treated explants (Fig. 6).

Fig. 6.

Fig. 6.

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Pillar cell shape is affected in blebbistatin-treated cochlear explants. (A) Low magnification view of a control explant established at E13 and fixed after 72 hours in vitro. The pillar cells (green) extend in a single line along the length of the explant. (B) Low magnification view of an explant established and labeled as in A, but treated with 10 μM blebbistatin for 48 hours beginning after 24 hours in vitro. The overall length of the epithelium is shorter and the row of pillar cells appears less organized. (C) High magnification view of the sensory epithelium from a control explant labeled as in A. The pillar cells are present in a single organized row. (D) The same view as in C with the red channel removed. Pillar cells are indicated (arrows). (E) High magnification view of the sensory epithelium from an explant treated with 10 μM blebbistatin, labeled as in A. (F) The same view as in E, with the red channel removed. Note the poor organization of the row of pillar cells and the more rounded shape. (G) Quantification of the average length and width of pillar cells in control and blebbistatin-treated explants. In blebbistatin-treated explants, pillar cell lengths are significantly shorter, whereas pillar cell widths are significantly greater, resulting in a significant decrease in the length/width ratio. Scale bars: 100 μm in A (same magnification in B); 20 μm in D (same magnification in C,E,F).

Myosin II-dependent extension occurs between E14.5 and E17.5

As discussed above, previous results had suggested that a considerable amount of cochlear convergence and extension occurs between E14 and E16.5. To determine whether the effects of myosin II are limited to this phase of development, cochlear explants were established at E13.5 and treated with blebbistatin for 48 hour time periods beginning after 0, 1, 2 or 4 days in vitro (equivalent to E13.5, E14.5, E15.5 or E17.5; Fig. 7A,B). All explants were fixed after a total of 6 days in vitro. Also, as it was difficult to bisect the cochlea in exactly the same place in each explant, cochleae were established intact and the full extent of the Reissner's membrane was removed to completely expose the sensory epithelium. The presence of an intact sensory epithelium did not appear to significantly affect extension, however, the average width of the sensory epithelium was somewhat wider by comparison with explants that had been bisected (data not shown). Significant shortening and widening of the sensory epithelium was observed when blebbistatin treatment was initiated at either E14.5 or E15.5 (Fig. 7C,D). Initiation of blebbistatin treatment at E13.5 did not lead to a significantly shorter sensory epithelium (Fig. 7C), possibly because myosin II-dependent outgrowth does not begin prior to E14.5. By contrast, treatment with blebbistatin between E17.5 and E19.5 did not significantly affect cochlear length, but did result in a significant increase in the width of the sensory epithelium, suggesting that myosin II-dependent extension, but not cellular rearrangement, might be completed by E17.5. Regardless of the timing of blebbistatin addition, the total number of hair cells was unaffected.

Fig. 7.

Fig. 7.

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CE occurs autonomously within the sensory epithelium. (A,B) Control (A) and 10 μM blebbistatin (B) explants treated for 48 hours beginning at E14.5. Hair cells are labeled with anti-myosin 6, the sensory epithelium is shorter and wider in the blebbistatin-treated explant. (C,D) Lengths and widths for cochlear explants treated with 10 μM blebbistatin during the indicated time periods. Treatment beginning at E14.5 or E15.5 results in significant shortening and widening of the sensory epithelium. Treatment beginning at E17.5 results in a significant widening without a change in length. (E,F) Control (E) and 3 μM blebbistatin-treated (F) explants established without mesenchyme. The effects of blebbistatin are similar to those observed in explants with mesenchyme. (G,H) Effects of blebbistatin on the length and width of the sensory epithelium are comparable between explants with and without mesenchyme. Scale bar: 50 μm in A (same magnification in B,E,F). *P<0.05, **P<0.01, ***P<0.001.

Myosin II-dependent extension occurs autonomously in the cochlear epithelium

The results described above suggest that myosin II provides the driving force for extension within the cochlear sensory epithelium. However, in vitro explants also contained mesenchymal cells located beneath the basement membrane of the developing sensory epithelium. Since these cells have been implicated in several aspects of cochlear development, including outgrowth (Phippard et al., 1999), it seemed possible that the outgrowth of the sensory epithelium could be an indirect result of ongoing extension in the associated mesenchyme. Therefore, to determine whether extension of the sensory epithelium occurs autonomously, cochlear explants were established as described in the previous section, with the exception that all underlying mesenchyme was removed at the time of culture (Montcouquiol and Kelley, 2003). Treatment with blebbistatin still significantly inhibited both the lengthening and narrowing of the sensory epithelium (Fig. 7E-H), demonstrating that myosin II directly regulates extension within the sensory epithelium.

DISCUSSION

The results presented here demonstrate that extension between E14 and E16 plays a key role in cochlear patterning. During this time period, the length of the prosensory domain increases by ∼70% whereas the width of the domain decreases by ∼30%. Moreover, during the same time period, the lumenal surface of each prosensory cell increases by an average of 36%. As a result, prosensory cell density along the long axis of the cochleae decreases by nearly 50%. Since all prosensory cells are postmitotic at this point (Ruben, 1967) and cell death is minimal (Nikolic et al., 2000; Chen et al., 2002), the observed changes in patterning are most likely to be a result of cellular rearrangement. The demonstration that extension is disrupted in response to either genetic or pharmacological inhibition of myosin II indicates a crucial role for this molecule.

The specific morphological changes and cellular rearrangements that are mediated through myosin II are not clear. MYH10 and MYH14 are asymmetrically distributed between different cell types, as well as in different regions of individual cells. In particular, more intense labeling of MYH10 is present on cell membranes oriented parallel to the axis of extension. At these membranes it seems possible that MYH10 could play a role in the elongation of cells along this axis. Results in both Dictyostelium and Xenopus have suggested that myosin II, and in particular myosin IIB (MYH10) plays a key role in regulating changes in cell shape through its role as an actin crosslinker (Egelhoff et al., 1996; Laevsky and Knecht, 2003; Rolo et al., 2009). Morpholino-based inhibition of myosin IIB in Xenopus neural tube leads to defects in neural tube closure as a result of defects in cell shape change (Rolo et al., 2009). Similar defects were observed in these studies, suggesting a potential similar role for myosin II in the cochlea.

In addition, mutations in zipper (Drosophila myosin II) have been shown to lead to disruptions in the formation of boundaries in the imaginal disc and ommatidia (Major and Irvine, 2006; Fiehler and Wolff, 2007), and mutations in Myh10 in mice lead to hydrocephalus as a result of disruptions in the ventricular layer boundary (Ma et al., 2007). MYH10 and MYH14 are distributed at boundaries between different cell types within the OC, and the alignments of these cell types was affected in blebbistatin-treated explants and, to a lesser extent, in Myh10DN mutants. The specific role of myosin II in boundary formation is unclear. However, its ability to regulate contractile tension along F-actin cables through crosslinking has been implicated (Major and Irvine, 2006; Ma et al., 2007).

Myosin II has also been shown to regulate CE during germband extension in Drosophila through modulation of junctional remodeling (Bertet et al., 2004; Zallen and Wieschaus, 2004). In particular, cell-cell junctions oriented perpendicular to the axis of extension are actively eliminated, whereas junctions oriented parallel are actively developed or increased. The distribution of MYH proteins in the developing cochlea was inconsistent with a similar role for myosin II in junctional remodeling. However, the changes in the distribution of pillar cells in cochleae in which myosin II function was perturbed suggest that some amount of junctional remodeling does occur.

Short cochleae and cellular patterning defects are also observed in animals with mutations in PCP genes, such as Vangl2 or dishevelled (Montcouquiol et al., 2003; Wang et al., 2005; Wang et al., 2006). The similarities in the phenotypes suggest that PCP and myosin II could function in the same signaling pathway. This possibility is supported by data indicating interactions between PCP and myosin II in Drosophila ommatidial rotation (Winter et al., 2001). Conversely, CE in the developing Drosophila germband is dependent on myosin II but is apparently not regulated through the PCP pathway, as Frizzled and Dishevelled are not required for extension in this system (Zallen and Wieschaus, 2004). This raises the possibility that the similar cochlear phenotypes are not a result of perturbations in a single pathway and instead occur because of disruption of distinct pathways that result in similar phenotypes. Shortened cochleae have also been observed in humans with Mondini dysplasia, often caused by mutations in the anion transporter SLC26A4 (Campbell et al., 2001), and in mice in response to targeted removal or disruption of multiple genes expressed within the inner ear, including Foxg1, neurogenin 1, Pou3f4 and Gli3 (Phippard et al., 1999; Ma et al., 2000; Pauley et al., 2006; Qian et al., 2007; Bok et al., 2007). None of these genes has been implicated in PCP, suggesting that other pathways mediate other aspects of cochlear elongation. At this point, it is not possible to determine whether myosin II functions through a PCP-dependent or independent pathway, however, analysis of myosin II distributions in PCP mutants will be informative.

One of the more intriguing results of this study was the observation that morphological changes consistent with convergence and extension were largely restricted to the developing IPC and outer hair cell regions (compare changes in Fig. 3 with those described in Bertet et al. (Bertet et al., 2004). These results suggest that cochlear extension is probably asymmetric. Convergence apparently occurs predominantly, or exclusively, from the lateral side, with all cells moving towards a boundary that is established between the inner hair cells and IPCs.

In conclusion, the results presented here demonstrate a role for myosin II in the outgrowth and patterning of the developing sensory epithelium, as well as in changes in the shape and size of the lumenal surface areas of individual prosensory cells. MYH10 and MYH14 are distributed in patterns that are suggestive of multiple roles in cochlear development, including CE and the establishment of cell-cell boundaries. In addition, disruptions in myosin II activity through either genetic or pharmacological methods result in shorter cochleae with marked defects in cellular patterning. Finally, analysis of changes in cell shape and position indicate that cellular convergence within the sensory epithelium is not symmetric, with more pronounced changes in cell shape occurring in the lateral (IPC and outer hair cell) region. These results identify myosin II as a key regulator of cellular patterning within the cochlea and provide intriguing new insights into the morphological changes that are required for the development of this rigorously patterned epithelium.

Supplementary material

Supplementary material for this article is available at http://dev.biologists.org/cgi/content/full/136/12/1977/DC1

Supplementary Material

[Supplementary Material]
supp_136_12_1977__index.html (4.2KB, html)

The authors wish to acknowledge the excellent technical assistance of Weise Chang. This project was supported by funds from the NIH Intramural program to R.S.A. and M.W.K. and by grants from the JSPS Research Fellowship for Japanese Biomedical and Behavioral Researchers at NIH to N.Y. and T.O. Deposited in PMC for release after 12 months.

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Supplementary Materials

[Supplementary Material]
supp_136_12_1977__index.html (4.2KB, html)
supp_136_12_1977__1.pdf (81.2KB, pdf)
supp_136_12_1977__2.pdf (281.7KB, pdf)
supp_136_12_1977__3.pdf (140.6KB, pdf)
supp_136_12_1977__4.pdf (81.8KB, pdf)

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