ErbB Expression: The Mouse Inner Ear and Maturation of the Mitogenic Response to Heregulin
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- Hume, C.R., Kirkegaard, M. & Oesterle, E.C. JARO (2003) 4: 422. doi:10.1007/s10162-002-3008-8
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In humans, hair cell loss often leads to hearing and balance impairments. Hair cell replacement is vigorous and spontaneous in avians and nonmammalian vertebrates. In mammals, in contrast, it occurs at a very low rate, or not at all, presumably because of a very low level of supporting cell proliferation following injury. Heregulin (HRG), a member of the epidermal growth factor (EGF) family of growth factors, is reported to be a potent mitogen for neonatal rat vestibular sensory epithelium, but its effects in adults are unknown. We report here that HRG-α stimulates cell proliferation in organotypic cultures of neonatal, but not adult, mouse utricular sensory epithelia. Our findings support the idea that the proliferative capabilities of the adult mammalian vestibular sensory epithelia differ significantly from that seen in neonatal animals. Immunohistochemistry reveals that HRG-binding receptors (erbBs 2–4) and erbB1 are widely expressed in vestibular and auditory sensory epithelia in neonatal and adult mouse inner ear. The distribution of erbBs in the neonatal and adult mouse ear is consistent with the EGF receptor/ligand family regulating diverse cellular processes in the inner ear, including cell proliferation and differentiation.
Keywordsauditoryvestibularhair cell regenerationgrowth factorcochleaproliferation
The vertebrate inner ear contains multiple types of sensory hair cells that are responsible for the detection of sound and motion. In birds, if the sensory epithelium is damaged, supporting cell precursors are stimulated to proliferate and differentiate into new hair cells (Corwin and Cotanche 1988; Ryals and Rubel 1988; Weisleder and Rubel 1993). As these new hair cells are reinnervated, this efficient and highly ordered process results in the restoration of auditory and vestibular function (reviewed in Cotanche et al. 1994; Carey et al. 1996; Stone et al. 1998; Cotanche 1999; Smolders 1999). In contrast to birds, mammals are unable to regenerate auditory hair cells and have a very limited ability to regenerate vestibular hair cells via a mitotic pathway if the sensory epithelium is damaged (Warchol et al. 1993; Lambert 1994; Rubel et al. 1995; Tanyeri et al. 1995; Li and Forge 1997; Zheng and Gao 1997; Kuntz and Oesterle 1998a; Forge et al. 1998).
Little is known about the signals that regulate the regeneration of hair cells. Despite the testing of extensive numbers of known growth factors by several groups, factors capable of stimulating proliferation in the mammalian auditory epithelium, the organ of Corti, have not yet been identified. Only a few factors show some promise of increasing proliferation and promoting new hair cell formation in the mammalian vestibular sensory epithelium (reviewed in Staecker and Van de Water 1998; Oesterle and Hume 1999). The most effective of these, epidermal growth factor (EGF) (Yamashita and Oesterle 1995; Zheng et al. 1997, 1999), transforming growth factor alpha (TGF-α) (Lambert 1994; Yamashita and Oesterle 1995; Zheng et al. 1997, 1999; Kuntz and Oesterle 1998a; Oesterle et al. 2003), glial growth factor 2 (GGF2) (Montcouquiol and Corwin 2001), heregulin (HRG) (Zheng et al. 1999), and neu-differentiation factor (NDF) (Gu et al. 1998, 1999), are structurally related members of the EGF-ligand family. GGF2, HRG, and NDF are also members of the neuregulin family, a subfamily of the larger EGF-ligand family that consists of over 15 splice isoforms arising from a single gene, NRG1.
The most studied of these ligands in the inner ear to date, TGF-α, has been shown to stimulate supporting cell proliferation in cultured utricular sensory epithelium from neonatal rats and adult mice (Lambert 1994; Yamashita and Oesterle 1995; Zheng et al. 1997, 1999). TGF-α’s mitogenic effects are potentiated by insulin (Yamashita and Oesterle 1995; Kuntz and Oesterle 1998a), and TGF-α plus insulin infusion into the adult rat ear stimulates the production of new supporting cells, and possibly new hair cells, in the utricular sensory epithelium in vivo (Kuntz and Oesterle 1998a; Oesterle et al. 2003). EGF, when used in combination with insulin, also stimulates supporting cell proliferation in an in vitro organotypic culture system from adult mice (Yamashita and Oesterle 1995) and in isolated sheets of neonatal utricular sensory epithelium (Zheng et al. 1997, 1999).
Several members of the neuregulin family, GGF2, NDF, and heregulin (HRG) β, are mitogenic for neonatal vestibular sensory epithelia (Gu et al. 1998, 1999; Zheng et al. 1999; Montcouquiol and Corwin 2001). In the adult, their effects are unknown (NDF, HRG) or incompletely characterized (GGF2, Gu et al. 1997). HRG-β appears to be a potent mitogen for neonatal vestibular sensory epithelia; a tenfold increase in the numbers of sensory epithelial (SE) cells synthesizing DNA was reported in cultures supplemented with HRG-β relative to that seen in control cultures (Zheng et al. 1999). Its effects need to be explored in adult tissues to determine its capabilities as a potential therapeutic agent for alleviating sensory-neural hearing loss or vestibular disorders in mammals, possibly in humans. The mitogenic effects of growth factors often vary developmentally in many tissues; hence, factors that are mitogenic for neonatal inner ear sensory epithelia may not necessarily have similar effects in adult tissues.
As summarized in Figure 1, signaling by members of the EGF family of ligands is mediated by four interacting transmembrane tyrosine kinase receptors: erbB1 (EGFR, HER), erbB2 (HER2, neu), erbB3 (HER3), and erbB4 (HER4) (for review, see Carraway and Cantley 1994; Lemke 1996; Burden and Yarden 1997; Riese and Stern 1998; Adlkofer and Lai 2000). The erbB receptors differ in both their ligand affinity and signaling activity. ErbB receptor family members, with the exception of erbB2, bind multiple ligands. Ligand binding induces receptor dimerization and activation of the intrinsic tyrosine kinase followed by activation of downstream signaling pathways. Receptor dimerization can take place between identical receptors (homodimers) or with any of the other erbB family members (heterodimers), depending on which receptors are expressed in a given cell (Riese et al. 1996a, b; Sliwkowski et al. 1994). ErbB2 does not have an identified ligand, but it is frequently activated as a result of receptor heterodimerization (Alroy and Yarden 1997; Sliwkowski et al. 1994). ErbB3 is an unusual receptor in that it does not possess any kinase activity, although it can recruit other receptors to form active heterodimers (Guy et al. 1994).
There are three functional groups of EGF-related ligands based on their ability to bind individual erbB receptors (Fig. 1) (reviewed in Riese and Stern 1998). One group of ligands (EGF, TGF-α, and amphiregulin) binds to receptors containing erbB1 (EGFR). The second group, the neuregulins (NRGs1–4), including HRG, binds to receptors containing erbB3 or erbB4, and the third group [betacellulin (BC), heparin-binding EGF (HB-EGF), and epiregulin (EPR)] binds to receptors containing either erbB1 or erbB4.
We examined the mitogenic effects of HRG-α in organotypic cultures of normal, undamaged utricular macula taken from neonatal (P3–P5) and adult mice (4–6 weeks). HRG-α was found to stimulate DNA synthesis in neonatal, but not adult, utricular macula. Immunohistochemistry and immunofluorescence revealed that erbBs 1, 2, 3, and 4 are widely expressed in the neonatal vestibular sensory epithelia and organ of Corti. We also show that erbBs 1, 2, 3, and 4 are expressed in distinct, but overlapping, subsets of cells within the adult mouse ear. The distribution of erbBs in the neonatal and adult mouse ear is consistent with the EGF receptor/ligand family regulating diverse cellular processes in the inner ear, including cell proliferation, differentiation, survival, and motility. The limited proliferation of mammalian inner ear sensory epithelia in response to EGF family members does not appear to be due to the lack of erbB receptor expression.
MATERIALS AND METHODS
Animal care and sacrifice were conducted according to methods approved by the University of Washington Animal Care Committee. Adult (4–12 weeks old) mice (Swiss Webster) were sacrificed by cervical dislocation (for cultured tissue only) or by anesthesia with CO2 followed by cervical dislocation. Postnatal day (P) 1–5 mice were sacrificed by decapitation.
Recombinant human heregulin-α (EGF domain; amino acid residues 177–241; Catalog No. 296-HR) was purchased from R & D Systems (Minneapolis, MN).
Previously described culture techniques (Yamashita and Oesterle 1995) were employed. After decapitation, heads were immersed in ice-cold 70% alcohol and transferred into sterile cold Hanks Balanced Salt Solution (HBSS). The utricles were isolated and placed free-floating into wells of 24-well tissue culture plates (one utricle per well) filled with 2 ml of Basal Medium Eagle (BME) (GIBCO, Rockville, MD) supplemented with Earle’s Balanced Salt Solution (EBSS) (GIBCO; BME:EBSS = 2:1), 0.5% glucose (Sigma, St. Louis, MO), and 0.1% fetal bovine serum (Atlanta Biologicals Inc., Norcross, GA). To test the efficacy of the HRG-α isoform on proliferation, 5, 25, 50, and 100 ng/ml of HRG-α was added to the experimental cultures at the beginning of the culture period. Growth factor was not added to the control cultures, which were otherwise cultured identically to the experimental cultures. Five-bromo-2′-deoxyuridine (BrdU; Sigma) was added to all cultures at 1 µM at the start of the culture period to identify cells that passed through S phase. Utricles were cultured for 6 days at 37°C in 5% CO2/95% air, immersion fixed in 4% paraformaldehyde in 0.1 M phosphate buffer (pH 7.4) for 20 min, and processed for immunofluorescence for BrdU and a hair cell-specific marker as described below. Three to four experimental runs were conducted (3 for adults, 4 for neonatals), and four to ten organs per experimental paradigm were studied.
Paraffin and cryostat sections
The temporal bones from adult mice were dissected free in ice-cold HBSS. After removal of the bulla, the stapes was gently lifted from the oval window, cochleostomies were made at the apical and basilar turns, and the semicircular canals were transected. Ice-cold, fresh 4% paraformaldehyde in 0.1 M phosphate buffer, pH 7.4, was then perfused slowly through the cochlea, and the temporal bones were transferred to fixative overnight at 4°C. Temporal bones were decalcified at room temperature in 0.4 M EDTA (pH 8.0) 1% paraformaldehyde for up to 5 days with daily solution changes. Mouse retinae, used as positive controls, were prepared in an identical fashion. The tissue was prepared in one of three ways for immunohistochemical processing: (1) half-temporal-bone preparations, (2) paraffin sections, or (3) cryostat sections. Specifically, to obtain half-temporal-bone preparations, decalcified temporal bones were bisected along the modiolar axis using an ultrathin razor blade and processed for immunohistochemistry as described below. To obtain paraffin sections of the inner ear, decalcified temporal bones were dehydrated with a graded ethanol series, cleared in methyl salicylate, and infiltrated with Paraplast Plus at 60°C. The entire inner ear was sectioned transversely at 3–6 µm and sections were mounted onto glass slides. To obtain cryostat sections of the inner ear, decalcified temporal bones were immersed in 30% sucrose in phosphate-buffered saline (PBS) overnight. The temporal bones were placed in O.C.T. compound (Miles Laboratories), frozen rapidly with dry ice, and cut into 10-µm sections with a cryostat. Sections were mounted onto ethanol/HCL chrome-alum-subbed slides and processed for immunohistochemistry as described below.
The brains from neonatal mice were removed, and the heads were immersed in fixative (4% paraformaldehyde in 0.1 M phosphate buffer, pH 7.4) overnight, or for 2 h in some experiments. After washes in PBS, the temporal bones were dissected free and processed as paraffin or cryostat sections as described earlier. Because the temporal bones of P1–P5 mice are not ossified, decalcification protocols were not used in these experiments.
A panel of antibodies was used to detect EGF receptors. SC-03 (Santa Cruz Biotechnology, Inc., Santa Cruz, CA), a rabbit IgG raised against the C-terminus of human EGFR (identical sequence in mouse), was used at 1:250 to detect erbB1. Western blot analyses carried out by the manufacturer on murine samples have demonstrated that the Santa Cruz SC-03 antibody (as well as the Santa Cruz erbB2 sc-284, erbB3 sc-285, and erbB4 sc-283 antibodies discussed below) does not cross react and recognizes a single protein of the correct size. To detect erbB2, two antibodies were tested, SC-284 (Santa Cruz; rabbit IgG raised against amino acids 1169–1186 of human erbB2) and RB-103-P1 (NeoMarkers, Union City, CA; rabbit anti-erbB2 polyclonal antibody raised against amino acids 1243–1255 from human erbB2). The SC-284 antibody was used routinely (at 1:500) to detect erbB2. The following three antibodies were used to detect erbB3: (1) SC-285 (Santa Cruz; rabbit IgG raised against amino acids 1307–1323 of human erbB3) was used at l:250; (2) Ab-236, polyclonal rabbit sera specific for the ligand-binding domain of erbB3 (against amino acids 71–86) (kindly provided by Dr. Nita Maihle, Mayo Foundation, Rochester, MN), was used at 1:1000; and (3) an affinity-purified Ab-236 antibody (provided by Dr. Nita Maihle) was used at 1:1000 (Lee and Maihle 1998). To detect erbB4, three antibodies were tested, but two (0616 and 0618) were used routinely. The 0616 and 0618 antibodies (kindly provided by Dr. Cary Lai, Salk Institute) were rabbit IgG raised against different epitopes of the cytoplasmic tail of erbB4, and they were used at dilutions of 1:2500 (0616) and 1:5000 (0618). Antibody 0616 is directed against a sequence that corresponds to residues 1185–1238 in human erbB4 (Plowman et al. 1993); antibody 0618 is directed against a sequence that corresponds to residues 1108–1136 (Plowman et al. 1993). Western blot analyses of the 0616 and 0618 antibodies in mouse (Zhu et al. 1995) have demonstrated that the antibodies react specifically with erbB4 and not with erbB2 or erbB3. The 0616 and 0618 antisera gave similar staining patterns in control tissues and in the ear. SC-283 (Santa Cruz), a rabbit antiserum against human erbB4, was tested but not used routinely because it tended to give high background labeling of nuclei.
To label hair cells in neonatal mice, the following antibodies were used: anti-calretinin antibodies (Chemicon International Inc., Temecula, CA), mouse monoclonal (Catalog No. MAB1568) and rabbit polyclonal (Catalog No. AB149), were used at dilutions of 1:1000 or 1:2000; anti-parvalbumin (Sigma) mouse monoclonal used at a dilution of 1:1000 (Xiang et al. 1998); a rabbit anti-myosin VI polyclonal antibody (kindly provided by Dr. Tama Hasson, University of California–San Diego, La Jolla, CA) (Hasson et al. 1997) was used at 1:500. The myosin VI antibody was also used to label hair cells in adult mice.
A mouse anti-BrdU monoclonal antibody (Becton-Dickinson, San Jose, CA; Catalog No. 347580) was used at 1:100 to label cells as they passed through S phase.
Secondary antibodies were used at dilutions recommended by the manufacturer (1:200). Biotinylated goat anti-rabbit IgG and goat anti-mouse IgG were purchased from Vector Laboratories, Inc. (Burlingame, CA). Goat anti-rabbit IgG and goat anti-mouse IgG conjugated with fluorescent labels (Alexa 488, 568, 594, FITC, Bodipy-FL) were purchased from Molecular Probes (Eugene, OR), ICN (Costa Mesa, CA), and Vector Laboratories.
Immunohistochemical and immunofluorescent staining
BrdU/hair cell marker/bisbenzimide triple labeling
Utricles were incubated in 1 N HCl/0.1% Triton X-100 in PBS at 37°C for 30 min to denature DNA. After neutralizing washes in PBS (pH 8.5/pH 7.4), the tissue was treated for 3 h with 0.1% saponin/0.1% Tween 20 in PBS in order to make membranes more permeable to antibodies. Tissues were then incubated overnight in 10% normal goat serum/0.03% saponin/0.1% Triton X-100 in PBS. The following primary antibodies were added simultaneously: mouse anti-BrdU and either rabbit anti-calretinin (P3–P5 utricles) or rabbit anti-myosin VI (4–6-week utricles) to label hair cells as described above. The primary antibodies were diluted in 3% normal goat serum/0.03% saponin/0.1% Triton X-100 in PBS, and the tissues were incubated overnight at 4°C. After three 15-min washes with 0.1% Tween 20 in PBS, tissue was incubated simultaneously with both fluorescently labeled secondary antibodies for 4 h at room temperature in 3% normal goat serum/0.03% saponin/0.1% Triton X-100 in PBS. After 15-min wash in PBS with 0.1% Tween 20, the utricles were immersed for 15 min in the dark in bisbenzimide (Hoechst 33342, Sigma, 1:200) in order to label nuclei. Finally, the organs were washed (3 times for 10 min each) in PBS, placed on glass slides as whole mounts using 1% DABCO (Sigma) in glycerol, and coverslipped.
ErbB immunohistochemical staining
For the half-temporal-bone preparations, endogenous peroxidase activity was quenched by a 1-h incubation in 3% hydrogen peroxide, prior to antibody reactions. Primary and secondary antibody incubations were performed for 3–5 days each at 4°C in PBS, 0.03% saponin, 10% goat serum, 2 mg/ml bovine serum albumin, and 0.1% Triton X-100 with gentle agitation. Biotinylated secondary antibodies (1:200) were detected using the Vectastain Elite ABC kit (Vector Laboratories). Incubation with the ABC reagent was for 2 days. Bound antibody was visualized with 3–3′ diaminobenzidene (DAB). Stained temporal bones and retinae were embedded in Paraplast (Oxford Labware, St. Louis, MO) and sectioned.
Immunohistochemistry was also performed on paraffin and/or cryostat sections with the following modifications: (1) Endogenous peroxidase activity was quenched in 1% H2O2 for 30 min; (2) the primary antibodies were incubated with sections overnight at 4°C; and (3) secondary and ABC incubations were for 2 h at room temperature in the same buffers.
ErbB immunofluorescent staining
Paraffin or cryostat sections were prepared for immunofluorescence as described above, omitting the peroxidase-quenching step. Primary and secondary antibody incubations were performed for 1 day and 2 h, respectively, at 4°C in PBS, 0.03% saponin, 3% goat serum, 2 mg/ml bovine serum albumin, and 0.1% Triton X-100 with gentle agitation. Fluorescently labeled secondary antibodies (Alexa 488, 594, Molecular Probes) were used at a dilution of 1:200. In double-labeling experiments, sections were labeled simultaneously with both a rabbit anti-erbB antibody and a mouse anti-parvalbumin or anti-calretinin antibody (to identify hair cells). Fluorescent secondary antibodies were also incubated simultaneously in the double-labeling experiments. Sections were washed after each antibody incubation (3 times for 10 min each) in 0.1% Tween 20 in PBS. Sections were mounted in Vectashield (Vector Laboratories) and examined with epifluorescence.
For whole-mount labeling of utricles, otoconia were manually removed after fixation, and the utricles were incubated with primary antibodies as described for the half-temporal-bone preparations. Fluorescently labeled secondary antibody (Alexa 568, 594, 488 and Bodipy-FL, Molecular Probes) incubations were for 1–2 days at 4°C. After counterstaining nuclei with bisbenzimide (1 µg/ml), specimens were mounted in Vectashield and examined with either epifluorescence or confocal fluorescence microscopy.
Controls for immunohistochemistry/immunofluorescence
Method and antibody specificity were checked by (1) substituting nonimmune sera for the primary antibody, (2) blocking with the immunizing peptide when available (e.g., erbBs 1–3, Santa Cruz), (3) using a series of dilutions of the primary antibody, and (4) processing positive control tissues (mouse retina) alongside the inner ear tissue. Others have previously shown that erbB receptors have distinct tissue expression profiles in postnatal and adult rodent retina (Anchan et al. 1991; Lillien 1995; Bermingham–McDonogh et al. 1996). The specificity of these anti-erbB antibodies has been demonstrated previously in the adult rat and chinchilla inner ear (Matsunaga et al. 2001, Zhang et al. 2002). In double-labeling experiments, only antibodies raised in different species were used to avoid cross reactivity among the antibodies (e.g., mouse anti-BrdU was used with rabbit anti-calretinin). For both adult and neonatal animals, the antibody staining using immunofluorescent and immunohistochemical detection methods was consistent (not shown).
Whole-mount utricle preparations were viewed under epifluorescence on a Nikon Optiphot microscope with 10X (0.25 NA), 20X (0.4 NA) or 40X (0.65 NA) objectives, and images were captured with a Spot 2e camera (Diagnostics Instruments, Sterling Heights MI). The number of BrdU-labeled cells located within the sensory receptor epithelium, the utricular macula, was quantified for each utricle. The lateral borders of the sensory epithelium (i.e., sensory epithelium vs. transitional epithelium) are defined by the outermost hair cells (visualized by calretinin or myosin VI labeling). The bottoms of the supporting cell nuclei define the lower boundary of the sensory epithelium (sensory epithelium vs. underlying stromal tissues). All nuclei are labeled with bisbenzemide, and the densely packed supporting cell nuclear layer is easily discerned from the overlying, more sparsely packed hair cell nuclear layer and the underlying stromal tissue. The distinction between the sensory epithelial and stromal cell layers is rigorously maintained. We and others have previously shown that these layers can be routinely identified in whole-mount preparations based on the size, shape, and density of the labeled nuclei, as well as depth within the epithelium (Stone and Cotanche 1994; Warchol and Corwin 1996; Oesterle et al. 1997). Within the sensory epithelium, hair cell nuclei are larger in size and more spherically shaped than the smaller, oval-shaped supporting cell nuclei.
In the current studies, for each BrdU-labeled cell it was noted whether the labeled cell was double-labeled by the hair cell-specific marker and whether it occurred in a pair of BrdU-labeled cells, or as part of a cluster. Pairs of BrdU-labeled nuclei were defined as “two BrdU-labeled nuclei separated by a distance not more than twice the diameter of two nuclei.” Clusters of BrdU-labeled cells were defined as “three or more BrdU-labeled nuclei separated by a distance not more than twice the diameter of two nuclei.”
The area of each utricular macula was quantified by using Object Image 2.04e (written by Norbert Vischer, available from simon.biol.uva.nl), and the amount of BrdU labeling was expressed as the number of BrdU-labeled cells/mm2 of sensory epithelium (SE). Data from individual utricles were averaged to yield an average number of BrdU-labeled cells/mm2 SE for each experimental paradigm ± the standard error of the mean (SEM). Utricles with less than half of the SE (50,000 µm2) visible (e.g., as the result of tissue folding, an overlying flap of tissue, dissection damage, etc.) were excluded and were not included in the averages. Image enhancement and merging of images was performed with Adobe Photoshop 5.5 (Adobe, Seattle, WA).
Significance values were determined with one-way analyses of variance (ANOVAs), and two-group comparisons were determined with t tests or with the Mann–Whitney U test (StatView 5.0, SAS Institute, Inc., Cary, NC). Post hoc comparisons, where appropriate, used the Fisher’s Protected LSD, Duncan New Multiple Range, and Tukey–Kramer tests.
Heregulin-α stimulates proliferation in cultured utricular maculae from neonatal, but not adult, mice
We examined HRG-α’s effect on cell proliferation in the utricular macula of organotypic preparations of neonatal and adult mouse utricles. Utricles were cultured for 6 days in BrdU-supplemented medium (with or without test growth factor present), fixed, and immunofluorescently processed for BrdU and a hair cell-specific marker (calretinin or myosin VI) (e.g., Fig. 2A). Nuclei were counterstained with bisbenzimide (e.g., Fig. 2B).
A cultured control neonatal mouse utricle (no growth factor supplement) is shown in Figure 2A, B. Figure 2B is a higher magnification of the region in Figure 2A specified by the arrow. The green BrdU-labeled nuclei are easily distinguishable from the blue, bisbenzimide-labeled, non-BrdU-labeled nuclei. Few BrdU-labeled nuclei are seen in the sensory epithelium of the control utricle. An organ cultured identically to the control utricle, except that it was grown in the presence of 100 ng/ml HRG-α, is shown in Figures 2C and D. Figure 2D is a higher magnification of the region of Figure 2C specified by the arrow. A greater number of BrdU-labeled SE cells are present in the HRG-α-supplemented utricle than in the unsupplemented control.
The number of cells in the sensory epithelium synthesizing DNA during the 6-day culture period and macular area were quantitatively assessed in 7 unsupplemented (control) and 26 normal HRG-α supplemented utricles. The mean numbers of BrdU-labeled SE cells per utricle, or per mm2 SE, are listed in Table 1, and the mean numbers of BrdU-labeled cells/mm2 SE are shown in Figure 3. When these and other data are expressed as a function of SE area, it facilitates comparisons across species, as well as across different inner ear epithelia (e.g., vestibular vs. auditory). The neonatal utricular macula has a mean area of 101,084 µm2 (± 28,600 µm2 SD, n = 33). The addition of HRG-α increased the number of BrdU-labeled cells in a dose-dependent manner. While there were approximately 48.6 ± 19.8 SEM (n = 7) proliferative cells/mm2 SE in the control utricles, 353.9 ± 126.6 (n = 7) BrdU-labeled cells/mm2 SE were observed in the cultures supplemented with 50 ng/ml HRG-α. The addition of 50 ng/ml of HRG-α significantly increased (p < 0.05) the numbers of SE cells synthesizing DNA, a sevenfold increase was observed vis-à-vis controls. Labeled cells were found in both supporting cell and hair cell layers in control and HRG-α supplemented cultures. However, all BrdU-positive SE cells were calretinin negative, indicating that the proliferating cells did not acquire a hair cell phenotype by 6 days in culture. Most labeled cells were found in either pairs or clusters (Table 2), suggesting that many labeled cells are postmitotic pairs.
The HRG-α experiments were repeated on utricles from mature mice to determine whether the HRG mitogenicity was maintained in the mature sensory epithelium. Utricles from 4–6-week-old mice were cultured for 6 days in BrdU-supplemented medium in the presence or absence of HRG-α. The number of cells in the SE synthesizing DNA during the 6-day culture period and macular area were quantitatively assessed in 10 unsupplemented (control) and 20 HGR-α-supplemented utricles. The adult utricular macula has a mean area of 108,503 µm2 (± 29,147 µm2 SD, n = 30) and does not differ significantly in size from that of neonatal mice (p > 0.05). In contrast to the findings in neonatal mice, ongoing proliferation was not observed in the sensory epithelium of the mature mice; virtually no BrdU-labeled cells were seen (mean = 1.0 ± 1.0 SEM BrdU-labeled cells/mm2 SE; 1 labeled cell was seen in 10 utricular maculae) (Fig. 2E). Numbers of BrdU-labeled SE cells differed significantly (p < 0.01) in neonatal and mature control utricular maculae, demonstrating age-dependent differences in the amount of ongoing proliferation in mice utricles. Furthermore, in contrast to the findings in neonatals, addition of HRG-α (25, 50, 100 ng/ml) to mature utricular maculae did not potentiate SE cell proliferation (Fig. 3, Table 1).
Heregulin binding receptors are expressed in neonatal and adult inner ear
To determine whether downregulation of receptor expression was responsible for loss of the mitogenic response to HRG-α in the utricular sensory epithelium, we examined the distribution of erbBs in the inner ears of mice of comparable age to our culture experiments using immunohistochemistry/immunofluorescence and well-characterized polyclonal antisera specific for each receptor. We also examined erbB expression in the spiral and vestibular ganglia and in extrasensory tissues (spiral limbus, spiral ligament, stria vascularis, transitional epithelium) of adult mice.
Vestibular end organs
Adult: ErbB1 (EGFR) expression was examined in the vestibular end organs, and similar patterns of expression are found in the utricle, saccule, and cristae ampullaris. There is strong erbB1 labeling at the apical surface of the vestibular sensory epithelium that extends laterally into the extrasensory transitional zone lacking hair cells (Fig. 4A1). Supporting cells in both the otolithic organs and the cristae are immunoreactive for erbB1. ErbB1 labeling in the supporting cells extends from their apical processes at the reticular lamina down toward their bases that contact the basement membrane. In contrast, vestibular hair cells are unlabeled. This can be seen more clearly in an immunofluorescently stained whole-mount utricular preparation showing a rosette of labeled supporting cells surrounding an unlabeled hair cell (Fig. 4A2). Within the vestibular ganglion (Fig. 4B), erbB1 immunoreactivity is found in a subset of sensory neuron cells.
Neonatal: The supranuclear region of supporting cells in the vestibular sensory epithelia of P3–P5 mice is strongly labeled for erbB1 (Fig. 5A, B). Low levels of erbB1 label are present in the stroma (data not shown).
Organ of Corti
Adult: In the cochlea, erbB1 is expressed in both sensory and nonsensory cells. The strongest labeling is noted in Deiters’ cells and inner hair cells (IHCs) (Fig. 4D). In these cell types, the labeling appears to be distributed relatively uniformly from the basal to apical regions of the cells. Inner hair cell stereocilia are unlabeled. In contrast, in the pillar cells the labeling is not distributed uniformly; labeling of the apical portion of the stalks is more intense. ErbB1 labeling of outer hair cells (OHCs) is consistently more moderate than either IHC or Deiters’ cell labeling (Fig. 4D). Hensen’s cells are labeled more faintly than the neighboring Claudius’ cells (data not shown). Immunoreactivity for erbB1 is also present in other nonsensory cell types, such as the inner sulcus cells (data not shown), the interdental cells of the spiral limbus (Fig. 4E), cells of the spiral ligament (Fig. 4C), and Reissner’s membrane (Fig. 4E). ErbB1 labeling is absent from the stria vascularis and basilar membrane. The tympanic border cells that line the underside of the basilar membrane and face the scala tympani are faintly labeled for erbBl (Fig. 4D). When comparing apical and basal turns of the cochlea, no consistent differences were found in the level of erbB1 immunoreactivity in either sensory or extrasensory cells. Within the spiral ganglion (Fig. 4F), erbB1 labeling is found in the majority of sensory neuron cells.
Neonatal: ErbB1 is expressed in supporting cells in the basal and apical turns of the neonatal organ of Corti (P3–P5) (Fig. 6A). The strongest labeling is found in the supporting cells immediately lateral to the OHCs (Hensen’s/tectal cell region) and the pillar cells. Immunoreactivity for erbB1 is also present in the cells of the greater epithelial ridge.
Vestibular end organs
Adult: ErbB2, like erbB1, is expressed in the vestibular periphery. We consistently find labeling of the reticular lamina in the sensory receptor epithelia of each of the vestibular organs (cristae, saccule, and utricle). Transitional epithelial cells bordering the sensory epithelium are also labeled (Fig. 7A1). In the ampullary organs, erbB2 labeling of hair cells was observed (Fig. 7A2). The labeling of the stereocilia was also seen in control tissue. The cell bodies of many sensory neurons in the vestibular ganglion are also strongly labeled for erbB2 (Fig. 7B).
Neonatal: ErbB2 antibodies label vestibular supporting cells in sensory epithelia of P3–P5 mice (Fig. 5C, D). Apical and basal regions of the supporting cell cytoplasm are labeled and the supporting cell nuclei are unlabeled.
Organ of Corti
Adult: ErbB2 immunoreactivity is detected in both sensory and nonsensory cell types in the adult organ of Corti. The strongest labeling is found in the IHCs (Fig. 7D). ErbB2 labeling is absent from IHC stereociliary bundles and nuclei. Immunoreactivity for erbB2 is found at moderate levels in Deiters’ cells, the spiral ligament, and in Claudius’ and outer sulcus cells (Fig. 7C). Boettcher’s cells are also immunopositive (data not shown). Within the spiral ligament, the marginal region bordering the otic capsule shows strong labeling (Fig. 7C). These cells may correspond to tension fibroblasts or bone-lining cells (Henson and Henson 1988; Chole and Tinling 1994). More moderate erbB2 immunoreactivity is found in the flbrocytes within the spiral ligament. Faint erbB2 immunolabeling is detected in the OHCs (Fig. 7D) and pillar cell heads. Similar to erbB1, the labeling of erbB2 within OHCs has a punctate quality, and the OHC nuclei and stereocilia are unlabeled. Like erbB1, erbB2 labeling is absent from the stria vascularis and basilar membrane (Figs. 7C, D). No significant differences are seen when comparing erbB2 labeling between apical and basal turns of the cochlea. Within the spiral ganglion (Fig. 7F), fewer sensory neuron cell bodies are immunoreactive for erbB2 than erbB1.
Neonatal: Like erbB1, erbB2 labeling is strongest in the cells immediately lateral to the OHCs (Hensen’s/tectal cells) and in the pillar cells (Fig. 6C, D). No erbB2 immunoreactivity is found in hair cells at this age. As was seen with erbB1, faint erbB2 labeling is present in the cells forming the greater epithelial ridge.
Vestibular end organs
Adult: ErbB3 expression was detected in a subset of hair cells in the otolithic (Fig. 8A) and ampullary organs. Supporting cells were unlabeled, as was the transitional epithelium. Satellite cells in the vestibular ganglion are strongly labeled, and many vestibular ganglion neurons are moderately immunopositive (Fig. 8B).
Neonatal: In the vestibular sensory epithelia of P3–P5 mice, erbB3 immunoreactivity is present in the vestibular hair cells and supporting cells (Fig. 5E, F). A small subset of hair cells appears to label more strongly with erbB3 antibodies than adjacent hair cells (not shown).
Organ of Corti
Adult: In the adult organ of Corti, erbB3 immunoreactivity is seen in both supporting cells and hair cells (Fig. 8D). Outside of the sensory epithelium, Boettcher’s cells, outer sulcus cells, and inner sulcus cells also label for erbB3 (data not shown). Moderate erbB3 labeling is detected in the spiral ligament, but it is absent from the stria vascularis (Fig. 8C). Satellite cells in the spiral ganglion are strongly immunopositive for erbB3, whereas the neuron cell bodies are faintly labeled (Fig. 8F).
Neonatal: ErbB3 expression in the neonatal organ of Corti is shown in Figure 6E, F. ErbB3 immunoreactivity is seen in both supporting cells and in sensory hair cells with strong labeling of pillar and Deiters’ cells. Cells in the greater epithelial ridge are faintly immunoreactive (Fig. 6E, F), as are the nonsensory cells lateral to the organ (data not shown).
Vestibular end organs
Adult: Expression of erbB4 was also examined in the vestibular periphery. In the utricle, saccule, and cristae, type I and II hair cells and supporting cells are immunoreactive (Fig. 9A). ErbB4 is also present in transitional epithelial cells (Fig. 9A). Numerous vestibular ganglion cell bodies are immunoreactive for erbB4 (Fig. 9B). Similar results were obtained using the 0616 and 0618 antisera, although the signal was consistently stronger using 0616.
Neonatal: In P3–P5 vestibular sensory epithelia, erbB4 labeling resembles erbB3 labeling. Both hair cells and support cells are immunoreactive (Fig. 5G, H).
Organ of Corti
Adult: ErbB4 antibodies strongly label some organ of Corti cell types, namely in the head and stalk regions of the inner pillar cells (Fig. 9D). Granular erbB4 staining is also present in neural endings under the OHCs (arrow) and in the IHC region. Occasionally, supporting cells adjacent to the IHCs (e.g., border cells) are strongly labeled in the basal turn of the cochlea (data not shown). Basal cells of the stria vascularis are strongly labeled for erbB4 (Fig. 9C), whereas the spiral limbus is unlabeled (Fig. 9E). As can be seen in Figure 9F, moderate labeling for erbB4 is found in sensory neuron cells bodies within the spiral ganglion.
Neonatal: In the neonatal organ, moderate erbB4 labeling is present in hair cells and supporting cells (Fig. 6G, H). Faint erbB4 immunoreactivity is seen in the cells of the greater epithelial ridge. Moderate labeling is seen in some nonsensory cells lateral to the organ of Corti (Fig. 6G, H).
This study demonstrates the following: (1) There is spontaneous proliferation in cultured neonatal mouse vestibular sensory epithelium, whereas cell division is virtually nonexistent in adult mice; (2) the amount of proliferation in neonatal, but not adult, utricle cultures can be potentiated by heregulin-α, an EGF-related ligand; and (3) both neonatal and adult mouse inner ear express receptors for EGF-related ligands (erbBs) (including heregulin-α) in multiple cell types including support cells. A goal of research in the hair cell regeneration field is to develop therapies to alleviate sensorineural hearing loss and balance disorders resulting from hair cell loss. Our study shows a developmental difference in HRG mitogenicity not directly explained by receptor expression and emphasizes the importance of testing candidate growth factors in adult, as well as neonatal, animals.
Ongoing proliferation differs in neonatal and adult mice
The amount of proliferation that occurs in the neonatal (P2–P5) mouse utricular macula is orders of magnitude less than that of ongoing proliferation in the vestibular epithelium of birds (Jørgensen and Mathiesen 1988; Weisleder et al. 1995; Kil et al. 1997). Many (77%) of the BrdU-labeled cells we describe in cultured mouse utricular maculae are located in pairs or clusters of labeled cells, suggesting that they represent postmitotic pairs. None of the BrdU-labeled SE cells are double-labeled with the hair cell-specific marker calretinin. These data suggest that there are a few new supporting cells produced in the neonatal utricular maculae, but no new hair cells. Our findings are in agreement with the in vivo birthdating studies of Ruben (1967, 1969) in developing mouse utricle. Ruben reports that new hair cells are added from gestational day 12 (G12) through postnatal day 1 (P1) (not added at P3; P2 not studied), whereas supporting cell production continues a little longer, through P3 (not added at P5; P4 not studied).
In contrast to neonatal stages, virtually no DNA replication occurs in the adult (4–6 week) mouse macula. The numbers of labeled cells in neonatal utricular maculae were significantly different (P < 0.01) from those seen in adults. The very rare labeled cell that was seen in adults—one labeled cell in 10 utricular maculae—may be a proliferating leukocyte (Warchol 1997; Bhave et al. 1998; Oesterle et al. 2003).
A small amount of SE cell proliferation has been reported in organotypic cultures of adult guinea pig (Warchol et al. 1993) and mouse utricle (Lambert 1994). The small sample size (4 guinea pig utricles: Warchol et al. 1993; 2 mouse utricles: Lambert 1994) and possible surgical damage to the sensory epithelium makes it difficult to determine whether ongoing SE cell proliferation is present. Three to ten proliferating SE cells per cultured guinea pig utricle were reported by Warchol et al. (1993), but the proliferation appeared at sites of unintentional hair cell lesions that occurred during the surgical removal to culture. Proliferation was not detected in regions of the tissue that contained normal numbers of undamaged hair cells. The two mouse utricle cultures studied by Lambert (1994) contained 1 and 5 labeled SE cells. In organotypic cultures of adult (6–8 week) mice utricles, Yamashita and Oesterle (1995) did not detect significant ongoing proliferation in the utricular macula.
In addition to Ruben’s birthdating studies described above, several in vivo studies substantiate the low level of proliferation in the adult utricle. Kuntz and Oesterle (1998a) infused tritiated thymidine into normal adult rats for a 3- or 7-day period, and virtually no normal ongoing proliferation was seen in the utricular macula. Similarly, Li and Forge (1997) and Rubel et al. (1995) infused BrdU or tritiated thymidine into adult guinea pig ears over an extended period and ongoing proliferation was not detected in the utricular macula.
Heregulin-α increases proliferation in neonatal, but not adult, utricular macula
We find that HRG-α induces a sevenfold increase in proliferation in cultured utricular sensory epithelium of P3–P5 mice. No effect is seen when the utricular sensory epithelia from 4–6-week-old mice are cultured under the same conditions. These results confirm that HRG isoforms are mitogens for vestibular sensory epithelia of neonatal rodents, as was shown previously in rat (Zheng et al. 1999). Other studies have also identified growth factors mitogenic for neonatal inner ear sensory epithelia (e.g., Zheng et al. 1997, 1999; Gu et al. 1998, 1999; Montcouquiol and Corwin 2001). Our studies extend previous findings by showing that HRG does not induce proliferation in the sensory epithelia from mature mice.
The prototype EGF family members, EGF and TGF-α, that bind erbB1, have been shown previously to be mitogenic for adult vestibular sensory epithelia (Lambert et al. 1994; Yamashita and Oesterle 1995; Kuntz and Oesterle 1998a). In contrast, preliminary data suggest that the neuregulin GGF-2 is not mitogenic for isolated sheet cultures of P35 rat utricle (Gu et al. 1997). These data suggest that the mitogenic effects of the neuregulins, in contrast to TGF-α, may be limited to developing vestibular sensory epithelia.
In our studies using organotypic cultures of P3–P5 mouse utricle, the maximum (sevenfold) mitogenic effect of HRG-α was seen at 50 ng/ml. In neonatal rat, the maximum HRG-β effect was seen at 30 ng/ml in utricular epithelial sheet cultures, and a smaller mitogenic effect was seen in organotypic cultures (fivefold increase in SE cell proliferation) (Zheng et al. 1999). The fact that the maximum HRG-β effect is found at a lower concentration could either be due to a species difference (mouse vs. rat), a difference in culture techniques (epithelial sheets vs. whole utricle), or a difference between the two HRG isoforms. Heregulin-β binds the erbB3 and erbB4 receptors 100-fold more strongly than HRG-α (Jones et al. 1999). Although the β-isoform is known to be a more potent mitogen in several tissues, HRG-α is the most potent isoform in mammary epithelium in vivo (Jones et al. 1996). Hence, the effect of the two isoforms is not equivalent and may depend on receptor expression. Heregulin-α is expressed in supporting cells in postnatal rat and adult chinchilla utricular macula (Zheng et al. 1999, Zhang et al. 2002).
In neonatal animals, the magnitude of HRG’s mitogenic effects is smaller in organotypic explants (rat: fivefold increase, Zheng et al. 1999; mice: sevenfold increase, our data) than in isolated sheet cultures (rat: tenfold increase, Zheng et al. 1999). The discrepancies between organotypic and sheet cultures may be due to altered erbB expression resulting from the enzymatic and mechanical trauma to the sensory epithelium. Increased FGF receptor and IGF-1 receptor expression have been described in utricular macula sheet cultures relative to that seen in vivo (Zheng et al. 1997). The expression of many other genes is altered by enzymatic treatment and mechanical isolation of the sensory epithelium and this may affect growth factor responsiveness (Chen et al. 2001). In organotypic cultures, the sensory epithelium maintains its normal contact with the extracellular matrix and more closely resembles the in vivo ear.
The presence of erbB receptors in the SE and the reports of HRG-β’s mitogenic effects in isolated sheet cultures (Zheng et al. 1999) suggest that the mitogenic effect may be a direct effect. However, these sheet culture data must be interpreted cautiously because we show that the transitional epithelium, which borders the sensory epithelium, also expresses erbB receptors. Studies of Montcouquiol and Corwin (2001), using neonatal rat utricular sheet cultures where much of the transitional epithelium was removed, also support the idea that neuregulins can have direct mitogenic effects on the SE.
Supporting cells express erbB receptors
As described above, in vitro and in vivo studies have shown that the amount of proliferation induced in the vestibular sensory epithelium by members of the EGF family of growth factors (HRG, GGF2, and EGF) differs between adult and neonatal animals. To investigate the possibility that variation in receptor expression for these factors underlies the mammal’s limited ability to regenerate hair cells and its developmental regulation of proliferation, we characterized the expression of erbBs (1–4) in both adult and neonatal mouse inner ear by immunohistochemistry (see Tables 3 and 4). This allows a direct correlation of proliferation with expression of the relevant receptors in inner ear sensory epithelium from the same developmental age and species. Although all the major components of the adult inner ear are formed by birth, there is a dramatic postnatal cytological differentiation of the mouse inner ear. We also show that there are significant differences between erbB expression in adult and neonatal mice. In adult mouse vestibular end organs, strong erbB1 labeling is seen in the supporting cells. Interestingly, erbB1 appears to be expressed by all supporting cells in the sensory epithelia. Hence, the limited mitogenic effects seen with TGF-α (a ligand that preferentially activates erbB1 over other erbB dimers) are not the consequence of limited erbB1 expression in a subpopulation of supporting cells but must be the result of additional regulators of proliferation. We show that two additional receptors, erbB2 and erbB4, are also expressed in the vestibular supporting cells of adult mice. ErbB4 labeling is seen throughout the supporting cell cytoplasm, whereas erbB2 labeling is seen predominantly at the apical surface of the sensory epithelium. Like erbB1, erbB2 and erbB4 are expressed in all supporting cells in the vestibular sensory epithelia, not in a subset of cells. Expression of erbBs 1, 2, 4, and possibly erbB3, extends beyond the periphery of the vestibular sensory epithelium into the transitional zone. ErbB1 labeling in the transitional region is consistent with previous findings that TGF-α (Lambert 1994) and TGF-α plus insulin (Kuntz and Oesterle 1998b) induce proliferation in extrasensory regions, including the transitional epithelium.
In the adult cochlea, erbB1, erbB2, and erbB3 are expressed in Deiters’ cells, Hensen’s cells, and hair cells. ErbB3 is expressed in other organ of Corti supporting cells, including the pillar cells, inner phalangeal cells, and border cells. ErbB4, in contrast, has very limited expression in organ of Corti supporting cells but is expressed in nerve endings innervating the inner and outer hair cells. Extrasensory cells adjacent to the organ of Corti express erbB 1–3 receptors.
Several other groups have analyzed the expression of EGFR and erbBs in the mammalian inner ear. While the majority of studies were conducted in neonatal rats (Malgrange et al. 1998; Staecker et al. 1997; Zine and de Ribaupierre 1999; Zheng et al. 1999; Zine et al. 2000), limited data exist for the adult rat (Saffer et al. 1996; Zheng et al. 1999; Zine et al. 2000; Matsunaga et al. 2001; Daudet et al. 2002) and chinchilla (Zhang et al. 2002). Several of these studies have used RT-PCR techniques that do not provide detailed localization of erbB receptor expression within the labyrinth (Zheng et al. 1999; Saffer et al. 1996). Immunohistochemical techniques were used to characterize erbB expression in adult rat utricle and vestibular ganglion (Zheng et al. 1999; Matsunaga et al. 2001) and erbB1–4 expression in adult chinchilla inner ear (Zhang et al. 2002). The findings in chinchilla and rat appear to be largely consistent with our results in adult mice with several exceptions. In rat, each erbB is present in both the hair cells and supporting cells of the utricular macula (Zheng et al. 1999; Matsunaga et al. 2001). In adult chinchilla, erbBs 2, 3, and 4 are present in the auditory and vestibular sensory epithelia (Zhang et al. 2002). In contrast to mice, erbB2 and erbB3 are also reported to be present in the chinchilla stria vascularis (Zhang et al. 2002). Also, in contrast to our findings in mouse, erbB2 labeling is absent from spiral ganglion cells and minimal in IHCs. It has been suggested that this species difference may implicate erbB2 in the relative protection of mice from the ototoxic effects of carboplatin on the inner ear (Zhang et al. 2002). ErbB signaling involving erbB2 has also been shown to regulate the viability of adult rat vestibular ganglion neurons in vitro (Matsunaga et al. 2001).
Neonatal organ of Corti, like adult organ of Corti, is mitotically quiescent (Ruben 1967; Roberson and Rubel 1994; Sobkowicz et al. 1997; Zine and de Ribaupierre 1998; Zheng et al. 1999) and unable to repair itself after insult via a mitogenic pathway (Sobkowicz et al. 1992, 1996, 1997; Zine and de Ribaupierre 1998; Zheng et al. 1999). Exogenous application of EGF, TGF-α, or HRG-β1 fails to stimulate proliferation in organotypic cultures of neonatal rat organ of Corti (Zine and de Ribaupierre 1998; Zheng et al. 1999). The lack of responsiveness to the EGF family ligands does not appear to be due to an absence of receptors, as each erbB is widely expressed in the organ of Corti. Cells in the greater epithelial ridge also express all erbB receptors (1–4). Others have also analyzed erbB expression in the neonatal rat organ of Corti (Malgrange et al. 1998; Staecker et al. 1997; Zine and de Ribaupierre 1999; Zheng et al. 1999; Zine et al. 2000). As described above, some of these studies utilized PCR or ELISA techniques that do not provide cellular localization within the inner ear (Malgrange et al. 1998; Zine and de Ribaupierre 1999; Zine et al. 2000). In situ hybridization studies of neonatal rat organ of Corti localized erbB1 mRNA to hair cells, supporting cells (Deiters’ cells and Hensen’s cells), the greater epithelial ridge (Kölliker’s organ), and spiral ganglion cells (Zine et al. 2000). Immunohistochemical data from P3 rat organ of Corti suggest the presence of erbB1 in hair cell cytoplasm (Staecker et al. 1997), in stereocilia (Zine and de Ribaupierre 1999), on the surfaces of organ of Corti supporting cells, and at the apical junctions of cells in Kölliker’s organ (Zine and de Ribaupierre 1999). Our findings are in agreement with these earlier studies, except that we also see strong erbB1 labeling of cells in the Hensen’s/tectal cell region and moderate labeling of cells in the greater epithelial ridge. Unlike the immunofluorescence studies of P3 rat organ of Corti (Zheng et al. 1999), we do not see erbB2 labeling in neonatal mouse hair cells or Deiters’ cells. Like rat, we see label in mouse pillar cells and in the greater epithelial ridge.
Neonatal vestibular sensory epithelia, unlike neonatal organ of Corti, do not appear to be mitotically quiescent. As shown in this report, limited proliferation occurs normally in the undamaged neonatal vestibular sensory epithelium. Exogenous EGF family ligands, including EGF, TGF-α, GGF2, and HRG, are able to potentiate this proliferation (Zheng et al. 1977; Montcouquiol and Corwin 2001). We detected immunolabeling for all erbBs in supporting cells of neonatal mouse vestibular sensory epithelia. The localization of erbB receptors to the supporting cells is consistent with the mitogenic responsiveness of these cells to the EGF family ligands. Based on experiments using AG825, a specific inhibitor of erbB2, it has been hypothesized that GGF2’s proliferative effects are mediated through a receptor complex containing erbB2 (Montcouquiol and Corwin 2001).
Our findings in mice are in agreement with earlier studies in neonatal rat vestibular sensory epithelia (Zheng et al. 1999). PCR techniques were used to detect the presence of erbB2, erbB3, and erbB4 mRNAs in the utricular macula of P3 rats (Zheng et al. 1999). Previous immunofluorescence studies have also shown labeling for erbB2 in P3 rat utricle hair cells, supporting cells, and transitional epithelium (Zheng et al. 1999).
Several groups have generated targeted disruptions of the erbB1–4 genes in an attempt to understand the function of individual erbB receptors (Gassmann et al. 1995; Lee et al. 1995; Miettinen et al. 1995; Sibilia and Wagner 1995; Threadgill et al. 1995; Erickson et al. 1997; Riethmacher et al. 1997; Rio et al. 1997; Sibilia et al. 1998; Morris et al. 1999; Lin et al. 2000). No specific phenotype in the inner ear has been described for any of these strains. Analysis of these mice during embryogenesis and in adults may provide more information about the role of erbBs and their ligands in inner ear development and function.
In summary, we have shown that erbBs 1, 2, 3, and 4 are widely expressed to varying degrees in largely overlapping populations of cells within the neonatal and adult inner ear, including both sensory and nonsensory cell types. The expression of the erbBs in supporting cells, hair cells, and nonsensory cells suggests that they are potentially involved in the regulation of multiple processes, including survival, synaptic maintenance, and cochlear homeostasis, in addition to a role in proliferation. The expression of the receptors for TGF-α, EGF, and HRG does not appear to be the limiting factor for regulating proliferation within the sensory epithelium. Further characterization of the downstream signaling components of the erbB pathway may clarify the basis of our inability to induce robust hair cell regeneration in mammals.
The authors thank Dr. Tama Hasson for her gift of anti-myosin VI, Dr. Cary Lai for his gift of anti-erbB4 antibodies, Dr. Nita Maihle for her gift of anti-erbB3 antibody, Sidya Ty for excellent histological work, Glenn MacDonald for assistance with digital photography and imaging techniques, Dr. Jennifer Stone for helpful comments on the manuscript, Dr. Edwin Rubel for use of his laboratory facilities and his enthusiasm, and the anonymous reviewers. Supported by NIH/NIDCD grants DC03944 and DC04661 and the Oticon and American-Scandinavian Foundations.