Deaf‐blindness in three distinct genetic forms of Usher type I syndrome (USH1) is caused by defects in myosin VIIa, harmonin and cadherin 23. Despite being critical for hearing, the functions of these proteins in the inner ear remain elusive. Here we show that harmonin, a PDZ domain‐containing protein, and cadherin 23 are both present in the growing stereocilia and that they bind to each other. Moreover, we demonstrate that harmonin b is an F‐actin‐bundling protein, which is thus likely to anchor cadherin 23 to the stereocilia microfilaments, thereby identifying a novel anchorage mode of the cadherins to the actin cytoskeleton. Moreover, harmonin b interacts directly with myosin VIIa, and is absent from the disorganized hair bundles of myosin VIIa mutant mice, suggesting that myosin VIIa conveys harmonin b along the actin core of the developing stereocilia. We propose that the shaping of the hair bundle relies on a functional unit composed of myosin VIIa, harmonin b and cadherin 23 that is essential to ensure the cohesion of the stereocilia.
Usher syndrome (USH) is the most frequent cause of deaf‐blindness in humans. Three clinical subtypes, USH1–3, have been described (reviewed in Petit, 2001). USH1 is the most severe form. It is characterized by severe to profound congenital sensorineural deafness, constant vestibular dysfunction (balance deficiency) and pre‐pubertal onset retinitis pigmentosa. USH1 is genetically heterogeneous. Evidence for seven distinct genetic loci (USH1A–G) has been obtained, and four of the corresponding genes have been identified, namely USH1B, C, D and F (Petit, 2001; Mustapha et al., 2002). USH1B encodes the actin‐based motor protein myosin VIIa (Weil et al., 1995). USH1C encodes harmonin (Bitner‐Glindzicz et al., 2000; Verpy et al., 2000), a protein that contains PDZ domains (postsynaptic density, disc large, zonula occludens), modules known as organizers of submembranous protein complexes (Sheng and Sala, 2001). Alternatively spliced USH1C transcripts (Verpy et al., 2000) predict at least 10 protein isoforms which can be grouped into three subclasses, hereafter referred to as harmonin a, b, and c, and collectively as harmonin (Figure 1A). Finally, mutations in the genes encoding two cadherin‐related proteins, cadherin 23 and protocadherin 15, underlie USH1D (Bolz et al., 2001; Bork et al., 2001) and USH1F (Ahmed et al., 2001; Alagramam et al., 2001a), respectively.
Mouse mutants defective for myosin VIIa (shaker‐1) (Mburu et al., 1997), cadherin 23 (waltzer) (Di Palma et al., 2001) and protocadherin 15 (Ames waltzer) (Alagramam et al., 2001b) have been reported. They are all deaf and exhibit vestibular dysfunction. In these mutants, the sensory cells of the cochlea (the auditory organ) and vestibular end organs (balance organs) display anomalies in the development of their hair bundle. This mechanosensory structure is composed of an ensemble of 30–300 microvilli called stereocilia, that project from the apical surface of the hair cell (DeRosier and Tilney, 2000) (Figure 1B). As in other microvilli, stereocilia are tightly packed with actin filaments that are uniformly polarized and have their barbed end, i.e. their faster growing end, located at the tip (DeRosier and Tilney, 2000). However, stereocilia have several specific morphological features: (i) they are wider and longer than the microvilli of ‘conventional’ epithelial cells and can contain up to 2000 actin filaments in some species; (ii) they taper off at their base, where they insert into the apical surface of the cell, with only a few centrally located actin filaments extending through this region to anchor them into the cuticular plate (Figure 1B, right panel), a dense meshwork of cross‐linked actin filaments (DeRosier and Tilney, 1989); (iii) they are packed into rows of increasing height to form a highly organized and uniformly oriented hair bundle (Figure 1B); and (iv) they are connected by several different types of extracellular links (Pickles et al., 1984; Goodyear and Richardson, 1999). Upon deflection in response to the sound or acceleration stimulus, the stereocilia all pivot around their basal insertion points, causing opening or closing of the transduction channels, and thus fluctuations in the cell's membrane potential (Hudspeth, 1997).
With the exception of some studies addressing the role of myosin VIIa (Gale et al., 2001; Tuxworth et al., 2001; El‐Amraoui et al., 2002; Kros et al., 2002), the functions of the proteins underlying USH1 remain elusive. Here we address the role of harmonin in the inner ear. Because the three aforementioned mouse models of USH1 have disorganized hair cell stereocilia, and because harmonin, within the inner ear, is restricted to the sensory cells (Verpy et al., 2000), we hypothesized that this protein also is involved in the development of a coherent hair bundle. This prompted us to seek molecular partners of this protein. Our results implicate harmonin, cadherin 23 and myosin VIIa in a single functional network that underlies the formation of a coherent hair cell bundle.
Harmonin in differentiating hair cell stereocilia
We studied the distribution of harmonin during the period of hair bundle differentiation in the mouse and rat. In the mouse, stereocilia sprout from the apical surface of vestibular and cochlear hair cells at E13 and E15, respectively (Nishida et al., 1998; Denman‐Johnson and Forge, 1999). In the cochlea, hair cell differentiation proceeds from the base to the cochlear apex and, by P4–P6, the hair bundles reach their final adult shape (Nishida et al., 1998). A previous analysis of harmonin transcripts (see Figure 1A) has indicated that class b isoforms are restricted largely to the inner ear, whereas a and c forms have a much broader expression throughout the entire organism (Verpy et al., 2000). We thus focused our analysis on the b isoforms. Two polyclonal antibodies directed against the harmonin PST domain, that is only present in b isoforms, were generated. They both gave the same cellular distribution pattern. In the mouse vestibule, harmonin b was detected from E13 onwards, and it was restricted to the emerging stereocilia of the hair cells (Figure 1C and D). Detailed analysis by confocal microscopy showed that between E13 and E16, the harmonin b labelling delineated the entire length of the stereocilia (not shown). Likewise in the cochlea, harmonin b was first detected at E15 in the differentiating hair bundles of the basal turn hair cells. From E15 to E17, the immunoreactivity extended towards the cochlear apex. From E16 in the vestibule (Supplementary figure 1A and B, available at The EMBO Journal Online) and P0 in the cochlea, the protein became concentrated at the apex of the maturing stereocilia (Figure 1E–I and data not shown). From P30 onwards, harmonin b was no longer detected in the cochlea. In the vestibule, the labelling only persisted in a few sensory hair cells, in both type I and type II hair cells (not shown). In contrast to the harmonin b expression profile, an antibody that recognizes an epitope common to the three harmonin isoform classes (a, b and c) detected the proteins both in the cuticular plate and along the stereocilia (Figure 1G–I), during the embryonic and postnatal life of the animal.
Harmonin b is an F‐actin‐bundling protein
To address the function of harmonin, a representative of each of the three isoform classes was first transfected into HeLa cells. In cells producing harmonin a (Figure 2A) or harmonin c (not shown), the protein was distributed uniformly throughout the cell body. In contrast, in cells expressing harmonin b, the protein was associated with filamentous structures (Figure 2B). Double immunolabels with antibodies to α‐tubulin, β‐tubulin, cytokeratin 18, vimentin or a pan cytokeratin antibody showed that harmonin b was not associated with microtubules or intermediate filaments (not shown). Rather, harmonin b was co‐localized with actin filaments labelled with rhodamine–phalloidin (Figure 2B–D). To determine which domain(s) of harmonin b interact with the actin cytoskeleton, several truncated versions of the protein were expressed in HeLa cells. The shortest harmonin b fragment that co‐localized with the actin filaments encompasses the second coiled‐coil domain through the C‐terminal end (CC2‐Cter, amino acids 405–859) of the protein (not shown). In transfected cells, harmonin b‐labelled structures were observed as either punctiform or long and curvy filaments (Figure 2B–D). Using three‐dimensional spatial analysis, we found that the former are present almost exclusively at the cell plasma membrane–substrate interface, whereas the latter extended up to 10 μm throughout the cell, both being distinct from the actin stress fibres. We then studied the dynamics of green fluorescent protein (GFP)–harmonin b distribution in HeLa cells by digital fluorescence microscopy. The harmonin b label was first observed 6 h after transfection. At this stage, the protein was restricted to and highly concentrated at the distal end (barbed ends) of actin fibres, where they anchored to substrate adhesion sites (Figure 2E–J). Vinculin, a major component of the focal adhesion plaques (Zamir and Geiger, 2001) (Figure 2E, F and H–J), overlapped with the distal part of the harmonin b staining (Figure 2H and I). Observations performed at different intervals from 8 to 48 h after transfection indicated that harmonin b label extended further from the focal adhesion sites forming the long and curvy bundles. However, this changing pattern was slow as we observed only moderate modification of harmonin b‐labelled structures in cells analysed by time lapse during a 4 h interval (not shown). To characterize further the behaviour of actin filaments in the presence of harmonin b, cells were treated with either latrunculin A (Figure 3B), which binds to and sequesters actin monomers, or cytochalasin D (Figure 3C), that binds to the barbed end of actin filaments and alters actin polymerization. With either of these drugs, both the cortical actin filaments and the stress fibres were disrupted, whereas the curvy, harmonin b‐bound, actin filaments were unaffected (Figure 3A–C). Together, these results suggest that harmonin b stabilizes the actin filaments.
To determine how harmonin b interacts with F‐actin, we then carried out in vitro binding assays (see Materials and methods). Harmonin b and rhodamine–phalloidin‐labelled actin filaments were incubated together, and samples were visualized by light microscopy or were negatively stained for electron microscopy. We found that in the presence of the GST‐tagged CC2‐Cter harmonin b fragment (Figure 3D) or harmonin b (Figure 3E and F), actin filaments collected into large bundles. Upon GST cleavage by thrombin, the CC2‐Cter harmonin b fragment also promoted F‐actin bundling (Supplementary figure 3A). This actin‐bundling activity of harmonin b was not affected by a high calcium concentration (10 mM) or calcium chelating agents (10 mM EGTA) (not shown). To determine whether harmonin b associates with these actin bundles, we mixed the GST‐tagged CC2‐Cter harmonin b fragment with actin filaments to allow bundling, then the bundles were separated from soluble proteins and single actin filaments by low‐speed centrifugation. In the presence of the GST–CC2‐Cter harmonin, the vast majority of F‐actin was recovered in the pellet (Supplementary figure 3B). Finally, we demonstrated the direct binding of the CC2‐Cter harmonin b fragment to F‐actin by using CC2‐Cter‐ or GST‐coated beads incubated with actin filaments (Supplementary figure 3C and D). These results demonstrate that harmonin b has an actin‐bundling activity that is independent of calcium.
Cadherin 23 is present in the stereocilia and binds to harmonin b
Mutations of the gene encoding cadherin 23 cause USH1D in man. To study the distribution of cadherin 23 in the mouse developing inner ear, we raised three polyclonal antibodies against extracellular or intracellular regions of the protein (see Materials and methods). Just like harmonin b, cadherin 23 was detected along the entire stereocilia as soon as they emerge, and subsequently became restricted to their apical regions (Figure 4A–F), as confirmed by immunoelectron microscopy on P3 cochlear hair cells (Figure 4G and H). Both in the vestibule and in the cochlea, the temporal pattern was also identical to that of harmonin b. From P30, cadherin 23 was no longer detected in the cochlear stereocilia and only persisted in a few vestibular type I and type II hair cells. The disappearance of cadherin 23 from the stereocilia of adult mice indicates that the protein is not a component of the apical links of mature hair bundles.
The similar spatio‐temporal distributions of harmonin b and cadherin 23 in the stereocilia suggested that these molecules may interact. We therefore examined whether such an interaction could be detected in co‐transfected HeLa cells (Figure 5). In cells producing the cadherin 23 cytodomain (amino acids 3086–3354) and harmonin b, the two proteins entirely co‐localized throughout the cell cytoplasm (not shown). To determine whether cadherin 23 could recruit harmonin b to the cell membrane, we analysed its distribution in the presence of the hEcad–cad23 chimeric protein. The hEcad–cad23 protein is composed of the extracellular and transmembrane domains of Ecadherin directly linked to the cytodomain of cadherin 23 (Figure 5A). In HeLa cells producing the two proteins, the hEcad–cad23 chimera was detected at the cell–cell contacts, where it recruited harmonin b. In contrast, harmonin b was absent at cell–cell contacts lacking the hEcad–cad23 chimera (Figure 5B). Moreover, the presence of hEcad–cad23 modified the harmonin b–actin pattern, i.e. long harmonin b‐bound curvy filaments changed into punctate labelled structures (Figure 5B; Supplementary figure 5), thus suggesting an association between harmonin b and cadherin 23. Pull‐down assays were then performed. Extracts of transfected HEK293 cells producing either harmonin a, harmonin b or the myosin VIIa tail (amino acids 848–2215) were incubated with immobilized GST‐tagged cadherin 23 cytodomain (amino acids 3086–3354) or GST alone. Harmonins a and b were recovered with the GST‐tagged cadherin 23 cytodomain, but not with GST alone. In contrast, the myosin VIIa tail was not recovered (Figure 6A). The interaction between cadherin 23 and harmonin was analysed further by an in vitro binding assay (Figure 6B). Different harmonin fragments were produced (see Materials and methods) and incubated with immobilized biotin‐tagged cadherin 23 cytodomain. Both the PDZ1–PDZ2 peptide (amino acids 138–403) of harmonin and the PDZ2 domain alone (amino acids 189–307) bound to the cadherin 23 cytodomain, whereas binding was not observed with either PDZ1 or PDZ3 (Figure 6B and E).
These findings were confirmed by the results of a yeast two‐hybrid screening. The last 268 amino acids of the cadherin 23 cytoplasmic domain were used as a bait to screen exhaustively a P2–P6 inner ear sensory epithelium cDNA library. Eighteen independent clones encoding harmonin were found to bind specifically to the cadherin 23 cytodomain. The overlapping sequences of these clones, amino acids 114–322, map to the PDZ1 and PDZ2 domains of harmonin (Supplementary figure 6A). Together, these results demonstrate that harmonin, via its PDZ2 domain, binds to cadherin 23.
Harmonin b binds to myosin VIIa and is mislocated in myosin VIIa‐deficient mice
Myosin VIIa was recently shown to be a bona fide motor protein that moves along actin filaments (Udovichenko et al., 2002). Although the directionality of myosin VIIa movement along actin filaments has not been determined, all myosins (except for myosins VI and IXb) tested to date are actin plus end directed (Berg et al., 2001; Inoue et al., 2002). We thus addressed the possibility that myosin VIIa tows proteins towards the plus ends of actin filaments near the stereocilium tip. To this end, we studied the distribution of cadherin 23 and harmonin b in Myo7a4626SB shaker‐1 mice which carry a premature stop codon in the motor domain of myosin VIIa, and have severely disorganized hair bundles (Mburu et al., 1997). In both the vestibular (Figure 7A–C, G and H) and cochlear (Figure 7D–F and I–K) hair cells from E20 to P30, we failed to detect harmonin b in the stereocilia. Instead, harmonin b was found to be organized in a circle of bead‐like foci located around the periphery of the cuticular plate (Figure 7A, H and I). In contrast, harmonin a/c (Figure 7F) and cadherin 23 (Figure 7J) were both present in the stereocilia and distributed as in wild‐type mice. Likewise, two other proteins of the stereocilia, namely espin, an actin cross‐linking protein (Zheng et al., 2000), and stereocilin, a protein of as yet unknown function (Verpy et al., 2001), were distributed normally throughout the length of the stereocilium in control and mutant mice (Figure 6K and data not shown). These results suggest that myosin VIIa is involved in the transport of harmonin b up to the tip region of the stereocilium.
Such a proposal implies that the myosin VIIa tail and harmonin b physically interact. In co‐transfected HeLa cells producing harmonin b and either the entire myosin VIIa tail or its C‐terminal MyTH4 + FERM repeat (amino acids 1750–2215), we observed that the myosin VIIa fragments entirely co‐localized with harmonin b and actin (Supplementary figure 6B; data not shown). Moreover, the presence of the myosin VIIa fragments profoundly modified the harmonin b–actin pattern, just as the cadherin 23 cytodomain did. Similar co‐transfection experiments with harmonin a or c led to similar results, thus arguing in favour of an interaction of the three harmonin subclasses with myosin VIIa (data not shown). Because purified harmonin b was not stable, we tested the binding of harmonin a to myosin VIIa by in vitro binding assays. The C‐terminal MyTH4 + FERM repeat of myosin VIIa did interact with GST‐tagged harmonin a, and with GST–MyRIP (myosin VIIa and Rab‐interacting protein) used as a positive control (El‐Amraoui et al., 2002)), whereas it failed to bind to GST alone (Figure 6C) or GST‐tagged cadherin 23 cytodomain (not shown). In contrast, the ezrin FERM domain did not bind to GST–harmonin a (Figure 6C). By using various constructs expressing PDZ domains of harmonin b, we showed that only PDZ1 has affinity for myosin VIIa (Figure 6D and E).
A yeast two‐hybrid screen corroborated these results. Using a C‐terminal fragment of the myosin VIIa tail containing the SH3, MyTH4 and FERM domains (amino acids 1605–2215) as the bait, six independent clones encoding harmonin were isolated from our inner ear two‐hybrid cDNA library. Their overlapping sequences encode a harmonin fragment (amino acids 90–368) containing PDZ1, PDZ2 and part of the CC1 domain (Supplementary figure 6C). Together, these results demonstrate that harmonin, via its PDZ1 domain, interacts with the myosin VIIa tail.
In this study, we addressed the developmental role of harmonin in the inner ear sensory cells (hair cells). Mutations in the gene, USH1C, encoding this PDZ domain‐containing protein have been shown to underlie one genetic form of USH1 (Bitner‐Glindzicz et al., 2000; Verpy et al., 2000). Here, we show that harmonin directly interacts with cadherin 23, a protein defective in another genetic form of USH1 (Bolz et al., 2001; Bork et al., 2001). We also show that harmonin b, which thus far has only been detected in the inner ear (Verpy et al., 2000), binds to actin filaments. In addition, cadherin 23 and harmonin b concomitantly appear in the emerging stereocilia and disappear from the adult hair bundle. Together, these results strongly suggest that harmonin b bridges cadherin 23 to the cytoskeletal actin core of the stereocilium. Since Cdh23 mutations result in the disorganization of the hair bundle, and cadherin 23 is a member of the cadherin superfamily of cell–cell adhesion molecules, it has been proposed that this protein may cross‐link the stereocilia (Di Palma et al., 2001). Here, we show that cadherin 23 is present at the surface of the growing stereocilia, whereas it is absent from the hair bundles of adult mice. Therefore, cadherin 23, via homophilic interaction, is likely to form transient lateral links that interconnect the stereocilia from their emergence up to their final maturation. As a consequence of its extended extracellular region (27 cadherin repeats) and as proposed for the related FAT cadherin (Cox et al., 2000), cadherin 23 may also function as a sensor that detects cell membrane proximity in its microenvironment. Thereby, cadherin 23 could initiate contact between adjacent stereocilia.
The extracellular region of classical cadherins (e.g. Ecadherin) consists of five repeats. Adhesion between neighbouring cells is mediated by the homophilic interaction of the cadherin extracellular domains that form dimers in trans, and cluster, in a calcium‐dependent manner (Angst et al., 2001; Jamora and Fuchs, 2002). Ecadherins only provide weak cell–cell adhesion unless they are bridged to the actin cytoskeleton. The formation of adherens junctions involves the dynamic and regulated assembly of its molecular components (Gumbiner, 2000; Angst et al., 2001; Jamora and Fuchs, 2002). The cytodomain of Ecadherin binds to β‐catenin, which recruits α‐catenin that interacts with actin filaments (Yap et al., 1997; Imamura et al., 1999). The α‐ and β‐catenins are actually absent from the growing hair bundle (A.El‐Amraoui, unpublished results). Furthermore, cadherin 23 lacks the consensus R1 and R2 binding sites for β‐catenin (Imamura et al., 1999) but possesses the C‐terminal tri‐peptide class 1 consensus binding site for a PDZ domain, S/T‐X‐Φ (where X is any amino acid and Φ is hydrophobic) (Sheng and Sala, 2001). Further studies are required to determine whether cadherin 23 binding to harmonin is mediated through this C‐terminal tripeptide (TEL). Our results reveal a novel mode of association between a member of the cadherin family and the cytoskeleton, via the binding of the cadherin cytodomain to a PDZ domain‐containing protein, harmonin b, that directly interacts with F‐actin. The cadherin 23–harmonin b–actin filament complex is expected to strengthen the cohesion between stereocilia, by anchoring cadherin 23 to the actin core, initially along the entire length of the growing stereocilia and eventually in the more mature hair bundle, at discrete apical sites. In addition, the F‐actin‐bundling property of harmonin b that we show in vitro suggests that harmonin b is implicated in the dynamics of the stereocilia actin core in the developing hair bundle. Two other actin‐bundling proteins, fimbrin and espin, have been identified in the stereocilia (Drenckhahn et al., 1991; Zheng et al., 2000). However, unlike harmonin b, they distribute along the entire stereocilium and are present both in the developing and the adult stereocilia. The actin‐bundling activity of harmonin b, like that of espin and unlike that of fimbrin, is calcium independent. During hair bundle morphogenesis, harmonin b could contribute, as proposed for fimbrin and espin (Drenckhahn et al., 1991; Zheng et al., 2000), to the stiffness of the stereocilia. Moreover, harmonin b‐bound actin filaments in HeLa cells exhibit a very unusual resistance to both cytochalasin D and latrunculin A, which suggests that harmonin b shifts the dynamics of actin filaments towards stabilization. Based on the dynamic expression pattern of harmonin b in the growing stereocilia, we propose that the protein stabilizes elongating actin filaments and, as growth ceases during late maturation, their barbed ends.
Our results also establish that myosin VIIa, an actin‐based motor protein (Udovichenko et al., 2002) which is defective in still another genetic form of USH1 (Weil et al., 1995), binds to harmonin in vitro. In shaker‐1 Myo7a4626SB mice with severely disorganized hair bundles, harmonin b is absent from the stereocilia. In these mutants, harmonin b remains associated with the periphery of the cuticular plate, where it may be associated with the actin filaments that make up this structure. Remarkably, this pattern is reminiscent of that observed transiently in normal development when the hair bundle starts growing (see insets Figure 1D). Therefore, in wild‐type mice, myosin VIIa is likely to be involved in the transport of harmonin b into the stereocilia up to its final location. We have shown previously that myosin VIIa binds to vezatin, a transmembrane protein of the hair bundle, which is closely associated with the ankle links (a subset of lateral links that interconnect the bases of adjacent stereocilia), and proposed that myosin VIIa, via its interaction with vezatin, acts locally to create a tension force between the actin core and the plasma membrane of the stereocilia; the same role would apply to the cell–cell junction where both myosin VIIa and vezatin are located (Kussel‐Andermann et al., 2000) as well as harmonin and cadherin 23 (data not shown). Based on this proposed function for the myosin VIIa–vezatin interaction, the abnormal gating of the mechanotransduction channels which has been detected in shaker‐1 Myo7a4626SB mice has been suggested to result from the defect of the force myosin VIIa may apply to the transduction channel (Kros et al., 2002). An alternative hypothesis should now be considered, namely that myosin VIIa indirectly modulates the gating properties of the channel by translocating regulatory proteins of the transduction process to the tip of the stereocilium. It is noteworthy that, unlike harmonin b, harmonins a and c were found along the entire length of the stereocilia even in the absence of myosin VIIa, thus indicating that myosin VIIa is dispensable for the transport of these isoforms into the stereocilia.
From the present functional characterization of har monin b, cadherin 23 and myosin VIIa, we propose the following molecular scenario in the developing hair bundle. Myosin VIIa first conveys harmonin b to its stereociliar location. There, harmonin b anchors cadherin 23‐containing interstereociliar links to the actin filament cores of growing stereocilia. In this respect, one should recall that at early stages of hair bundle development, the stereocilia do not have the actin rootlets that eventually anchor into the cuticular plate and are thought to contribute to bundle stability (Tilney et al., 1983). We suggest that the earliest connections between growing stereocilia are critical for shaping the hair bundle as a coherent unit, and that this relies on a cooperation between the three aforementioned proteins. A failure in this process would lead to the hair bundle disorganization observed in USH1 mouse models. Finally, an attractive hypothesis is that the functional network formed by harmonin b, cadherin 23 and myosin VIIa also implicates the proteins defective in the other genetic forms of USH1.
Materials and methods
Yeast two‐hybrid screenings
Microdissected vestibular sensory epithelia of 292 mice (aged from P2 to P6) were used to generate a random‐primed cDNA library (Rain et al., 2001). Screenings were performed using two different baits: the intracellular region of cadherin 23 (amino acids 3086–3354) and the C‐terminal fragment of myosin VIIa tail (amino acids 1562–2215), composed of SH3, MyTH4 and FERM domains.
A cDNA encoding the cytoplasmic region of cadherin 23 (NM‐022124; amino acids 3086–3354) was obtained by RACE‐PCR on a human retinal Marathon‐cDNA library. PCR products were subcloned into pCMV‐tag3B (Myc tag, Stratagene) and pcDNA (No tag, Invitrogen) for expression in HeLa cells, and into pGex‐4T1 (GST tag, Amersham) and pXa3 (biotin tag, Promega) for protein production. The mouse full‐length cDNAs encoding harmonin isoforms a1 (AF228924; amino acids 1–548), b2 (AY103465; 1–859) and c1 (1–403) were amplified from the inner ear cDNA library as a template and cloned into pCMV‐tag3C, pcDNA and pGex‐4T1. cDNAs encoding harmonin truncated forms, i.e. PDZ1–PDZ2 (amino acids 72–307), PDZ1 (72–88), PDZ2 (189–307) and PDZ3 (738–849), were subcloned into pCMV‐tag3C and pGex‐4T1. A human cDNA encoding the myosin VIIa tail (amino acids 847–2215) was cloned in pcDNA for expression in HeLa cells. For protein production, a zebrafish cDNA encoding His‐tagged myosin VIIa C‐terminal tail fragment (88.5% amino acid identity with the corresponding human fragment) was subcloned in the pFastBac HTa vector (baculovirus system, Life Technologies). hEcad–cad23 is a chimeric protein derived from two plasmids: (i) pcDNA3/hEcad‐Cαctn, provided by M.Lecuit (Institut Pasteur), in which the extracellular and transmembrane domains of human Ecadherin (hEcad) are fused to the C‐terminal 398 amino acids of α‐catenin (Cαctn); and (ii) pCMV‐cad23 containing the human cadherin 23 cytodomain (amino acids 3086–3354). The pcDNA3/hEcad‐Cαctn plasmid was digested by ClaI and XbaI to eliminate the α‐catenin fragment (all 398 amino acids). This fragment was then replaced by an amplified ClaI–XbaI fragment encoding the human cadherin 23 cytodomain (cad23; amino acids 3087–3354), thus giving rise to pcDNA3/hEcad–cad23.
The H3 polyclonal antibody was generated against a bacterially expressed peptide common to the three harmonin subclasses (PH3; amino acids 1–89). The H1b and H2b antibodies to harmonin b were generated against an epitope located in the PST domain of the protein (PHb: RTGDPGHPADDWEA; amino acids 636–649). Three different rabbit polyclonal antibodies against human cadherin 23 were generated: cad‐C against a peptide in the cadherin 23 cytodomain (Pcad‐C; amino acids 3324–3339), cad‐N against two peptides in the extracellular region, namely Pcad‐N1 (amino acids 1161–1174) and Pcad‐N2 (amino acids 2456–2470), and cad‐CN against all three peptides.
The specificity of the affinity‐purified antibodies was assayed by immunofluorescence and immunoblot analysis. Substitution of the pre‐immune sera for the purified anti‐harmonin or anti‐cadherin 23 antibody and pre‐adsorption of the antibodies with the corresponding antigens were used as negative controls.
Pull‐down and in vitro binding experiments
Transient transfections of HEK293 cells were performed using PolyFect Transfection Reagent (Qiagen) following the manufacturer's instructions. Cells were collected 2 days after transfection and processed for pull‐ down experiments as described (Kussel‐Andermann et al., 2000). The in vitro binding assays were performed using glutathione–Sepharose (Amersham), or Tetra‐link avidin resins (Promega) as described (Kussel‐Andermann et al., 2000). Briefly, to test harmonin–myosin VIIa interaction, a bacterial lysate containing the GST–harmonin fusion protein was incubated with glutathione–resin for 90 min at 4°C. The resins were washed with binding buffer (phosphate‐buffered saline with 5% glycerol, 5 mM MgCl2 and 0.1% Triton X‐100) supplemented with a protease inhibitor cocktail (Roche), and then incubated with the His‐tagged myosin VIIa, or a His‐tagged control protein, ezrin (amino acids 1–309) for 2 h at 4°C. The resins were washed four times with binding buffer supplemented with 150 mM NaCl, and bound proteins were analysed by SDS–PAGE and immunoblotting, using the enhanced chemiluminescence (ECL) system (Amersham).
Immunofluorescence and electron microscopy analysis
HeLa cell lines were cultivated in 10% fetal calf serum (FCS)‐supplemented Dulbecco's modified Eagle's medium (DMEM). Transient transfections of these cells were performed using Effectene (Qiagen). Immunohistofluorescence analysis was carried out on fixed cells and cryostat sections of inner ears, as described (Kussel‐Andermann et al., 2000). Cells and tissue sections were analysed with a laser scanning confocal microscope (LSM‐510, Zeiss). For immunoelectron microscopy, cochleas from P3 mice (CD1 strain) were labelled with affinity‐purified cad‐N anti‐cadherin 23 antibodies or, as a control, non‐immune rabbit IgG (Goodyear and Richardson, 1999).
The following mouse monoclonal antibodies were used: anti‐Myc (clone 9E10) and anti‐His (Santa Cruz); anti‐GST (Amersham); anti‐vinculin (Sigma); and anti‐V5 (Invitrogen). For myosin VIIa detection in western blots, and harmonin–myosin VIIa double labelling experiments, a monoclonal mouse antibody (Farida‐Nato, IP), raised against a human myosin VIIa tail fragment (U39226; amino acids 905–1032), was used. Several polyclonal rabbit antibodies were used, which were directed against myosin VIIa (SSI) (El‐Amraoui et al., 1996), harmonin (NW2) (Kobayashi et al., 1999), espin (Zheng et al., 2000) and stereocilin (Verpy et al., 2001).
Actin binding assays
A 50 μM G‐actin solution (Molecular Probes) was polymerized by incubation for 30 min at 37°C in a high salt buffer containing 50 mM KCl and 2 mM MgCl2. A 10 μg aliquot of GST–harmonin b or GST–CC2‐Cter truncated form was incubated for 30 min with 15 μl of 10 μM F‐actin reconstituted from actin powder at 37°C. Actin polymers were either labelled with rhodamine–phalloidin and then observed under a fluorescence microscope, or analysed by electron microscopy after negative staining (Harris, 1991). Co‐sedimentation assays were done by mixing GST–CC2‐Cter harmonin b fragment with F‐actin, followed by centrifugation (30 min, 13 000 g). The same amounts of supernatant and pellet fractions were subjected to SDS–PAGE and analysed with the H1b anti‐harmonin antibody and Coomassie blue staining. For direct binding, glutathione–Sepharose beads coupled with GST or GST–CC2‐Cter harmonin b truncated form were mixed with 10 μM bundled F‐actin (F‐actin mix supplemented with 50 mM MgCl2). After three washes in high salt buffer, F‐actin was then visualized using rhodamine–phallodin.
Wistar Rats and RJ Swiss mice (Janvier, France) were used. Embryonic day 0 (E0) was determined by vaginal plug detection, and the day of birth was P0. The shaker‐1 Myo7a4626SB mice, obtained by ethylnitrosourea (ENU) mutagenesis, were kindly provided by Dr K.Steel (MRC, UK). Mice were genotyped as described (Self et al., 1998), and the absence of myosin VIIa was confirmed by immunohistochemistry using the anti‐myosin VIIa antibody. Twenty mutant mice at E20, P0, P2, P6, P10, P25, P30 and P60, with the same numbers of littermate controls, were analysed.
Supplementary data are available at The EMBO Journal Online.
We thank J‐P.Hardelin, P.Cossart and P.Herbomel for critical reading of the manuscript, J.Levilliers and D.Weil for their inexhaustible help, S.Ernest and M.Lecuit for the zebrafish myosin VIIa and hEcad–Cαctn chimeric constructs, and J.Bartles and I.Kobayashi for their kind gift of the anti‐espin and anti‐harmonin antibodies, respectively. This work was supported by grants from the EC (QLG2‐CT‐1999‐00988), the R. and G.Strittmatter Foundation, Retina‐France, the A. and M.Suchert, Forschung contra Blindheit—Initiative Usher Syndrom, Deutsche Forschungsgemeinschaft (Wo 548/3 and 4; U.W.), FAUN‐Stiftung (U.W.), Pinguin Stiftung (K.R.F. and U.W.) and The Wellcome Trust (057410/Z/99Z; G.R.). The confocal microscope was purchased with a donation from Marcel and Liliane Pollack. B.B. has a fellowship from Fondation pour la Recherche Médicale (France).
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