New Results

Dynamic coupling of cochlear inner hair cell intrinsic Ca2+ action potentials to Ca2+ signaling of non-sensory cells

Federico Ceriani, Stuart L. Johnson, Miloslav Sedlacek, Aenea Hendry, Bechara Kachar, Walter Marcotti, Fabio Mammano
doi: https://doi.org/10.1101/731851

ABSTRACT

The relationship between Ca2+ action potential (AP) activity in immature inner hair cells (IHCs) and the spontaneous ATP-dependent intercellular Ca2+ signaling in cochlear non-sensory cells (NSCs) of the greater epithelial ridge (GER) is unclear. Here, we determined that IHCs fired asynchronous Ca2+ APs also in the absence of Ca2+ activity in the GER. Patch clamp recordings from IHCs isolated from the rest of the sensory epithelium confirmed that this firing activity is an intrinsic property of immature IHCs. However, frequency, correlation index and burst duration of IHC APs increased significantly during Ca2+ wave propagation in NSCs, and depended on wave extension in the GER. Furthermore, IHC depolarization under whole cell patch clamp conditions triggered Ca2+ signals in nearby NSCs with a delay that was proportional to the distance from the stimulated IHC. Thus the immature mammalian cochlea supports bidirectional exchange of Ca2+ signals between IHCs and NSCs.

IMPACT STATEMENT In inner hair cells of the developing mammalian cochlea, Ca2+ action potentials are both intrinsic and bidirectionally coupled to the ATP-dependent Ca2+ signaling of the surrounding non-sensory cells.

INTRODUCTION

The primary sensory receptors of the mammalian cochlea, the inner hair cells (IHCs), fire Ca2+-dependent action potentials (APs) during pre-hearing stages of development (Kros et al., 1998; Beutner and Moser, 2001; Marcotti et al., 2003a; Johnson et al., 2011; Johnson et al., 2012; Johnson et al., 2017), which occurs at around postnatal P12 in mice (Mikaelian and Ruben, 1965; Shnerson and Pujol, 1981). During the same time window, periodic transient elevations of cytosolic free Ca2+ concentration occur spontaneously in the greater epithelial ridge (GER) and propagate as intercellular Ca2+ waves invading variable portions of the GER (Tritsch et al., 2007; Schutz et al., 2010; Rodriguez et al., 2012). The relationship between the AP activity in IHCs and Ca2+ signaling in the GER is still not fully understood (Mammano and Bortolozzi, 2018).

The GER comprises the tall columnar cells of Kölliker’s organ (Kikuchi and Hilding, 1965; Hinojosa, 1977) and all other cells of the sensory epithelium that are located on the modiolar side of the pillar cells, including the inner phalangeal cells, the border cells and the IHCs (Kelley, 2007). Connexin 26 (Cx26) and connexin 30 (Cx30) are the prevailing isoforms expressed in NSCs of the GER (Forge et al., 2003; Mammano, 2019) and their block prevents the generation of Ca2+ waves in the GER (Schutz et al., 2010; Xu et al., 2017; Mammano and Bortolozzi, 2018). Furthermore, intercellular Ca2+ wave propagation is hampered in Sox10-Cre;Gjb2fl/fl mice (Anselmi et al., 2008), with targeted ablation of Cx26 (Crispino et al., 2011), as well as in Cx30 homozygous knockout– LacZ mice (Gjb6−/−) (Anselmi et al., 2008; Ortolano et al., 2008; Rodriguez et al., 2012), both of which fail to acquire hearing (Teubner et al., 2003; Crispino et al., 2011; Fetoni et al., 2018). In contrast, intercellular Ca2+ waves propagate normally in mice that are global knockouts for pannexin 1 (Panx1–/–) (Zorzi et al., 2017; Mammano, 2019), and have hearing thresholds indistinguishable from those of littermate controls (Abitbol et al., 2019). Altogether, this evidence indicates that Ca2+ waves in the GER rely on ATP release from connexin hemichannels in the apical surface of NSCs (Tritsch et al., 2007; Schutz et al., 2010; Rodriguez et al., 2012; Xu et al., 2017; Mammano and Bortolozzi, 2018; Ceriani et al., 2019).

The ATP released during Ca2+ wave propagation has been proposed to trigger AP activity in immature IHCs, driving bursts of APs in the auditory nerve fibres (Tritsch et al., 2007). Extracellularly applied ATP caused elevation of cytosolic Ca2+ in adult IHCs (Dulon et al., 1991), due to activation of both ionotropic (P2X) and metabotropic (P2Y) purinergic receptors (Sugasawa et al., 1996). Immunolabeling experiments have demonstrated the presence of P2X2 purinergic receptors in the apical surface of IHCs, and shown to promote cell depolarization when activated by high concentrations of extracellular ATP (mature IHCs: Sugasawa et al., 1996; immature IHCs: Johnson et al., 2011). In contrast, ATP concentrations in the submicromolar range caused hyperpolarization in immature and mature IHCs, and this effect has been ascribed to a functional coupling between P2X receptors and SK2 channels (Sugasawa et al., 1996; Johnson et al., 2011).

Here, we used confocal Ca2+ imaging and patch clamp electrophysiology to provide an in depth investigation of the relationship between spontaneous AP activity in IHCs and intercellular Ca2+ waves in NSCs of the GER. Our results indicate that ATP-dependent signaling in cochlear NSCs is not required for AP generation in pre-hearing IHCs, but can increase the frequency of Ca2+ spikes in IHCs, thus increasing the probability of synchronized firing among nearby sensory cells.

MATERIALS AND METHODS

Ethics Statement

In the UK, experiments were performed in accordance with Home Office regulations under the Animals (Scientific Procedures Act) 1986 and following approval by the University of Sheffield Ethical Review Committee. In Italy, all experiments involving the use of animals (mice) were performed in accordance with a protocol approved by the Italian Ministry of Health (Prot. n.1276, date 19/01/2016). In the USA, experiments were conducted in accordance with the Guide for the Care and Use of Laboratory Animals by NIH and approved the Animal Care and use Committees for the National Institute on Deafness and Other Communication Disorders (NIDCD ACUC, protocol #1215).

Generation and genotyping of transgenic mice

For calcium imaging experiments in which genetically encoded calcium indicators were used, transgenic mice expressing GCaMP3 or GCaMP6f on the C57BL/6 background were utilized, bred to homozygosity and crossed with animals heterozygous for Gfi1-Cre (Yang et al., 2010) (hair cell only expression; MGI:4430258) or Emx2-Cre (Kimura et al., 2005) (whole epithelium expression; MGI:3579416). GCaMP3 knock-in mice (R26-lsl-GCaMP3) were a generous gift from Dwight E. Bergles (Johns Hopkins University), GCaMP6f mice (Madisen et al., 2015) were obtained from The Jackson Laboratory (B6;129S-Gt(ROSA)26Sortm95.1(CAG-GCaMP6f)Hze/J; Stock No.:024105; MGI:5558088). Transgenic animals were genotyped by standard PCR using specific primers for GCaMP3 and GCaMP6f animals, and generic Cre primers to genotype for Gfi and Emx2.

Tissue preparation

Ca2+ signaling and IHC activity in apical coil IHCs from wild type C57BL6/J mice of either sex were studied in either acutely dissected cochleae or in organotypic cultures from postnatal day 4-5 (P4-P5) pups, where the day of birth is P0. For organotypic cultures, cochleae were dissected in ice-cold Hepes buffered (10 mM, pH 7.2) HBSS, placed onto glass coverslips coated with 185 μg/ml of Cell Tak (Becton Dickinson) and incubated overnight at 37°C in DMEM/F12 (Thermo Fisher Scientific) supplemented with FBS 5%. Acute preparations were dissected in normal extracellular solution contained (in mM): 135 NaCl, 5.8 KCl, 1.3 CaCl2, 0.9 MgCl2, 0.7 NaH2PO4, 5.6 D-glucose, 10 Hepes-NaOH, 2 sodium pyruvate, amino acids and vitamins (pH 7.5; osmolality ∼308 mmol kg-1). Dissected cochleae were transferred to a microscope chamber, continuously perfused with a peristaltic pump using normal extracellular solution (see above) and viewed using an upright microscope (for microscope details, see Ca2+ imaging, below). Crucial for the generation of the AP activity in IHCs is the use of near physiological recordings conditions, which for the mammalian IHCs includes working at body temperature (35-37°C) and using a perilymph-like extracellular solution (1.3 mM Ca2+ and 5.8 mM K+) (Johnson et al., 2008; Johnson et al., 2017).

For experiments requiring the use of transgenic animals expressing Ca2+ biosensors, cochleae were dissected at room temperature in DMEM/F12 (Thermo Fisher Scientific) containing 10% fetal bovine serum (FBS) and ampicillin (5 µg/ml). After dissection, the tissue was mounted on a 10 mm glass cover slip coated with collagen and maintained in culture in a glass bottom Petri dish with DMEM/F12 at 37°C overnight. If cultures were kept in the incubator for another day, culturing media was exchanged 24 hours post dissection.

Electrophysiology

Patch pipettes were made from Soda glass capillaries (Harvard Apparatus Ltd, UK) and coated with surf wax (Mr Zoggs SexWax, USA) to minimize the fast transient due to the patch pipette capacitance. Recordings were made as previously described (Johnson et al., 2008; Corns et al., 2014; Johnson et al., 2017) using an Axopatch 200B (Molecular Devices, USA) or an Optopatch (Cairn Research, UK) amplifier. Data acquisition was controlled by pClamp software using Digidata boards (Molecular Devices, CA, USA). The cell-attached AP recordings were filtered at 10 kHz, sampled at 20 kHz and some were filtered offline at 500 Hz (8-pole Bessel) using Clampfit (Molecular Devices). Data analysis was performed using Origin software (OriginLab, Northampton, MA, USA). The pipette solution used for cell-attached recordings contained (in mM): 140 NaCl, 5.8 KCl, 1.3 CaCl2, 0.9 MgCl2, 0.7 NaH2PO4, 5.6 D-glucose, 10 Hepes-NaOH (pH 7.5). Hair cells spike occurrence was collected in peri-stimulus-time histograms. The Mini Analysis Program (Synaptosoft Inc. NJ, USA) was used to detect spike events in cell-attached recordings. The AP frequency was computed as the reciprocal of the mean interspike intervals (ISI) for each cell. To derive a continuous function for the firing rate vs. time, spike trains were smoothed by convolution with a Gaussian kernel (S.D. = 6 s).

Ca2+ imaging

For calcium dye loading, cochlear cultures and acutely dissected preparations from wild type animals were incubated for 40 min at 37°C in DMEM/F12, supplemented with fluo-4 acetoxymethil (AM) ester (final concentration 16 μM; Cat. No. F14217, Thermo Fisher Scientific). The incubation medium contained also pluronic F–127 (0.1%, w/v), and sulfinpyrazone (250 μM) (Sigma, UK) to prevent dye sequestration and secretion (Di Virgilio et al., 1989; Bootman et al., 2013). Preparations were then transferred on the microscope stage and perfused with extracellular solution for 20 minutes before imaging to allow for de-esterification. Fluo-4 signals were recorded using either a custom built spinning disk confocal microscope (Ceriani et al., 2016b) or a commercial two-photon confocal microscope (Ceriani et al., 2019).

For spinning disk confocal microscopy, Fluo-4 fluorescence was excited by light emitted from a 488 nm diode laser (COMPACT-150G-488-SM; World Star Tech), filtered through a narrow band filter (FF02-482/18-25, Semrock/IDEX Health & Science, LLC, Rocherster, N.Y.), and projected onto the sample by reflection off a 45° dichromatic mirror (Di02-R488-25×36, Semrock/IDEX Health & Science). Fluorescence emission was filtered through a OD6 bandpass interference filter (535/43M, Edmund Optics). Confocal fluorescence images were formed by a water immersion objective (40×, NA 0.8, LUMPLAFL, Olympus, Tokyo, Japan) and projected on a scientific–grade CMOS camera (Edge, PCO AG, Kelheim, Germany) controlled by software developed in the laboratory. Image sequences were acquired continuously at 10 Hz frame rate with 100 ms exposure time. To synchronize image acquisition and patch clamp recordings, we sampled the 5 V pulse (FVAL) that signals active exposure of the CMOS camera (Canepari and Mammano, 1999).

For multiphoton Ca2+ imaging with Fluo-4, a laser-scanning confocal microscope (Bergamo II System B232, Thorlabs Inc., Newton, New Jersey, USA) equipped with a water immersion objective, (60×, 1.1 NA, LUMFLN60XW, Olympus, Japan) was coupled to a mode-locked laser system (Chameleon Ultra II, Coherent Inc., Santa Clara, California, USA) operating at λ = 920 nm, 80 MHz pulse repeat, 140 fs pulse width. Fluorescence emission was filtered through a bandbass filter (FF02-525/40-25, Semrock/IDEX Health & Science) and detected by a cooled GaAsp PMT (H7422-40, Hamamatsu) to form raster-scan images (768×768 pixels) at 20 Hz frame rate.

For fluorescence imaging of GCaMP Ca2+ biosensors, we used an upright Nikon microscope equipped with Nikon water immersion objectives (either a 16× 0.8 NA CFI75 LWD, or a 25×C 1.1 NA CFI75 Apochromat), a Yokogawa CSU-21 spinning disc head, and an Andor DU-897 camera. For higher numerical aperture imaging, we flipped upside down the glass coverslip with the attached culture inside the glass bottom Petri dish and used drops of Vaseline as spacers. The upside down cultures (apical surface towards the objective) were viewed in a Nikon TiE inverted fluorescence microscope equipped with a Nikon objectives (either a 60×C 1.27 NA CFI SR Plan Apochromat IR water immersion objective, or a 100× 1.45 NA CFI Apochromat Lambda oil immersion objective), a Yokogawa CSU-21 spinning disc head, and an Andor DU-897 camera. NIKON Elements software was used for image acquisition. For pharmacology experiments, cultures were incubated with respective reagents for at least 20 minutes before imaging and then imaged in continuous presence of the drugs. Reagents were prepared fresh from stock solutions before each experiment.

Mathematical methods

Images were analyzed off-line using software routines written in MATLAB (Matlab R2011a, The Mathworks Inc.), Python (Python 2.7, Python Software Foundation) and ImageJ (NIH). Ca2+ fluctuations were quantified either as relative changes of fluorescence emission intensity Embedded Image or as normalized increments Embedded Image For the analysis in Figure 3, Ca2+ wave directions were estimated using an optical flow analysis algorithm (Afrashteh et al., 2017). First, each recording was preprocessed by applying a Gaussian (σ=2 pixels) and a median (2×2 pixels) filter. A ΔF/F0 image sequence was then generated from the raw data. Pixels belonging to different Ca2+ events were selected by drawing a ROI around the maximal extension of the wave. The processed recordings were then analyzed using Matlab and the Combined Local-global method of the Optical flow analysis toolbox (Afrashteh et al., 2017). We computed the distribution of instantaneous angles taken across all image frames of pixels within the ROIs. Finally, each wave was assigned to one of the three direction groups (IHCs to GER, GER to IHCs or longitudinal) based on the prevalent direction in the instantaneous angle distribution (IHC to GER: 225<α<315; GER to IHC: 45< α<135, longitudinal 135< α<225 and −45< α<45, where α is the angle between the optical flow vector and a line parallel to the IHCs, see Figure 3A).

Figure 1.
Figure 1. Optical detection of Ca2+-dependent action potentials in mouse cochlear IHCs.

(A) High magnification image of P5 cochlear IHCs loaded with Fluo-4 AM (see also Supplementary Video 1). (B) Representative traces showing optical detection of Ca2+ signals from the synaptic region of three adjacent IHCs. Traces were generated as pixel average from the three ROIs highlighted in (A). (C) Comparisons of cell-attached patch clamp recordings from a P5 IHC (top) and fluorescence Ca2+ signals from the same cell (middle). The bottom trace represents the time derivative of the fluorescence signal. Red bars single out APs detected by high-pass filtering of the patch clamp trace; downward triangles denote (corresponding) peaks of the ΔF/F0 trace. (D) Estimate of decay time constant from normalized fluorescence signals associated to individual Ca2+ action potentials. Temperature 34-37°C.

Figure 2.
Figure 2. Ca2+ waves propagate across GER non-sensory cells.

(A) Ca2+ waves that initiate in the proximity of inner phalangeal cells, which intercalate between IHCs, propagate both along the coiling axis of the cochlea (red ROIs and traces) and in the direction orthogonal to this (cyan ROIs and traces). (B) Kymograph corresponding to red traces in (A), showing repetitive Ca2+ waves that propagate along the L1 − L11 line. Note the nearly constant speed (slope) of these waves.

Figure 3.
Figure 3. Directionality of Ca2+ waves in the GER.

(A) Polar diagram superimposed to a reference fluorescence image of the organ of Corti. (B) Circle-chart showing the proportion of waves in each of the three directions (53 Ca2+ waves, 4 cochleae, 4 mice). (C-E) Polar histograms showing the distribution of instantaneous optical flow angles in three representative Ca2+ waves moving parallel to the tonotopic axis (C: longitudinal), from the IHC region towards the bulk of the GER (D) and from the GER towards the IHCs (E).

For correlation analyses (Figures 4-6), Ca2+ waves were identified using thresholding, and a region of interest (ROI) was drawn around the maximum extension of each multicellular Ca2+ elevation event. Only events that remained confined to the field of view of the microscope were considered for this analysis.

Figure 4.
Figure 4. Relation between IHC Ca2+ action potential and Ca2+ waves in non-sensory cells in the GER

(A,B) Representative recording of Ca2+ signals from 14 IHCs (blue) and non-sensory cells from four adjacent zones in the GER (cyan). (C) Correlation matrices computed from the IHCs in panel B. Correlation coefficients were computed in 5-s time windows in the absence (T1) or presence (T2) of Ca2+ waves in nearby non-sensory cells. (D) Correlation index between IHC activity as a function of Ca2+ wave area. Each data point represents the correlation index (average correlation coefficient) computed in a time window centered to the maximum amplitude of the Ca2+ wave (blue) or in the absence of Ca2+ waves in the GER (red). Filled dots: correlation index significantly different from 0 (P<0.05, Student’s t-test). Temperature 34-37°C.

Figure 5.
Figure 5. Modulation of IHC spontaneous activity by non-sensory cells

(A) Three representative frames from the same image sequence obtained while performing simultaneous Ca2+ imaging and cell-attached patch clamp recording from a P5 IHC. The top image shows the different regions of the sensory epithelium: the hair cell region (HCR) and the non-sensory cell region in the GER. The IHC was approached with the patch pipette from the outer hair cell side in order to avoid disruption the non-sensory cell in the GER. The IHC exhibited spontaneous electrical activity (white trace), the frequency of which increased when a Ca2+ wave was detected in nearby non-sensory cells (bottom panel). Scale bar: 25 μm. (B-D) Analysis of cross correlation between the IHC firing rate and Ca2+ signals in non-sensory cells. IHC burst frequency was significantly higher and burst duration was significantly longer when the firing was correlated with the occurrence of Ca2+ waves in proximal non-sensory cells.

Figure 6.
Figure 6. Spatial extent of IHC activity correlated with the occurrence of Ca2+ in the GER

Representative false-color image showing the spatial distribution of the cross correlation coefficient between Ca2+ transients in non-sensory cells and the firing rate of a patch-clamped IHC. Scale bar: 20 μm.

For the analysis in Figure 4, rolling (zero-lag) cross-correlation coefficients between different IHC Ca2+ traces were computed as: Embedded Image where x and y are two time series of size N, 2t is the size of the time window where the cross correlation was computed (5 seconds, or 100 frames) and Embedded Image are the average values of x and y in the time window. To estimate the correlation index (c), we first computed the rolling cross correlation for every pair of identifiable IHCs in the field of view (on average 14±2 cells per recording) in a time window centered on the peak of an intercellular Ca2+ wave. We then averaged these values using Fisher’s z-transformation (Fisher, 1915): z = arctanh(Ri), and its inverse c = tanh(z). Correlation index values are comprised between −1 and +1, with 0 indicating no correlation. This method was used also to estimate cross correlation coefficients between optical signals associated to GER Ca2+ waves and IHC firing rate, estimated from electrophysiological recordings (Figures 5 and 6). To this end, Ca2+ imaging datasets were first smoothed by applying a Gaussian (S.D. = 3 pixels) and median filter to every frame. Next, a baseline reference image (F0) was computed by averaging the first 5 frames of each recording. Time series were then generated by computing the pixel-by-pixel relative intensity change, ΔF/F0. To estimate the area of the GER were Ca2+ wave activity was significantly correlated to the spontaneous electrical activity of the patched IHC, we first down-sampled the IHC firing rate to the sample rate of the Ca2+ imaging acquisition. Then, a cross-correlation image was generated by calculating the cross correlation coefficient between the firing rate and the fluorescence values pixel-by-pixel. The background of this image was computed from an area of the GER that did not show any Ca2+ wave during the length of the recording. The longitudinal and radial extension of the correlation area was estimated using ImageJ.

For the analysis in Figure 5, IHC AP activity was considered significantly correlated to GER Ca2+ signaling activity when the cross-correlation coefficient was higher than a threshold that was determined using a Monte-Carlo approach by computing the (rolling) cross correlation of two pseudo-random traces having the same noise distribution as the original traces. The maximum value of the cross correlation coefficient was computed for 1000 different pairs of random traces, and the threshold was set at the 95% percentile.

For the analyses of GCaMP fluorescence signals in Figures 8 and 9, IHC activity was imaged and acquired using NIS-Elements software (Nikon Instruments, Inc.) at 0.5 – 2 Hz frame rate and analyzed later offline. Calcium transients were measured at the basal pole of contiguous IHCs, where single ROIs were manually set, as demonstrated in Figure 8B. Changes in fluorescence in IHCs during individual events were calculated as fluorescence of each event divided by the sum of total background fluorescence of the calcium indicator and event fluorescence (Fevent/Ftotal). Fluorescence profiles of each ROI/IHC were then plotted over time in NIS-Elements and numbers extracted to Igor Pro (Wavemetrics), where the fluorescence signals were translated into traces of raw fluorescence as shown in Figure 8D. Next, calcium transients were detected using a custom written derivative thresholding routine in Igor Pro that marked each detected event (see also (Zhou et al., 2018). Accuracy of detected events was verified by visual inspection. Frequency of events was calculated for each individual IHC as total number of detected events during the duration of a single trial and converted to frequency in Hz. Amplitudes were further analyzed and plotted in distribution histograms (0.02 Fevent/Ftotal bins) for each experimental and pharmacological condition (Figure 9A-C) and normalized relative to control (Figure 9D).

Figure 7.
Figure 7. IHC depolarization triggers Ca2+ waves in GER non-sensory cells

(A) Representative recording of membrane potential (black trace) and Ca2+ signals (blue trace) from an IHC a from a P5 mouse cochlea triggered by a series of 70 pA current injections under current clamp (2 s in duration, inset: see Materials and Methods) from the IHC resting membrane potential. (B) Representative frames from the same recording in panel A showing Ca2+ waves in proximal cochlear non-sensory cells of the GER triggered by each IHC depolarization. The temporal position of each frame is indicated by black arrows in panel A. Experiments were performed at 20-22°C in order to prevent or minimize spontaneous action potentials activity in IHCs.

Figure 8.
Figure 8. Expression and function of Ca2+ biosensors in the developing mouse cochlea.

(A-C) Representative confocal fluorescence images of cochlear culture from GCaMP3;Emx2-Cre mice (A), GCaMP3;Gfi1-Cre mice (B) and GCaMP6f;Gfi1-Cre mice (C); scale bars: 40 µm in (A) and (B), 40 µm in (C). (D) Detection of Ca2+ signals (events) from the basal pole of IHCs (see ROI examples in panel B) in one of these cultures based on time derivative computation of the raw fluorescence trace followed by thresholding.

Figure 9.
Figure 9. Pharmacological dissection of low- and large-amplitude Ca2+ transients in IHCs of mice expressing Ca2+ biosensors.

(A) Representative control records and corresponding amplitude distribution histogram; red traces: raw fluorescence data from a group of contiguous IHCs; black dots: events detected using the algorithm illustrated in Figure 8. (B) Effect of suramin. (C) Effect of thapsigargin. (D) Pooled data quantifying the effects of PPADS (100 µM), suramin (200 µM), ryanodine (50 µM), thapsigargin (10 µM) and nimodipine (50 µM); Ctrl, no treatment; DMSO, control to show lack of effect of the solvent (<0.1%) used for some of the water insoluble tested compounds; Data presented as means ± standard error of means (S.E.M); numbers of samples for each experimental condition are as follows: CTRL, n = 6; PPADS n = 4; Suramin, n = 3; ryanodine, n = 3; thapsigargin, n = 6; DMSO, n = 3. P-values (ANOVA) for each experimental condition relative to control for amplitude of detected events are as follows: PPADS, P = 1.34×10−4; suramin, P = 0.0032; ryanodine, P = 0.5549; thapsigargin, P =4.7607×10−5; DMSO, P = 0.8321. P-values (ANOVA) for each experimental condition relative to control for frequency of detected events are as follows: PPADS, P = 0.017; suramin, P = 0.0016; ryanodine, P = 0.7601; thapsigargin, P = 0.847; DMSO, P = 0.1374.

Statistical Analysis

Mean values are quoted ± S.E.M. (standard error of the mean). Two or more groups were compared by using two-tailed analysis of variance (ANOVA) or paired t test. The Mann-Whitney U test was used for data which were not normally distributed and/or had dissimilar variance. P-values are indicated by letter P, where P < 0.05 was selected as the criterion for statistical significance. Normality of distribution was determined using the Kolmogorov–Smirnov test.

No statistical methods were used to predetermine sample size. The experiments were not randomized and the investigators were not blinded to allocation during experiments and outcome assessment. No pre-established criteria were used to include/exclude samples or animals.

RESULTS

Optical detection of Ca2+-dependent APs in mouse cochlear IHCs

Spontaneous Ca2+-dependent activity in IHCs and NSCs in the GER was recorded from the apical coil of the immature mouse cochlea (P4-P5) bathed in a perilymph-like extracellular solution (1.3 mM Ca2+ and 5.8 mM K+: Wangemann, 1996) and at near body temperature. Under the above recording conditions, immature IHCs loaded with the Ca2+ indicator Fluo-4 AM exhibited spontaneous and rapid Ca2+ transients near their basal (synaptic) region (Figure 1A,B and Supplementary Video 1; similar Ca2+ transients were present in 10 separate recordings from 9 mice). By combining Ca2+ imaging and cell-attached patch clamp recordings, we confirmed that the observed Ca2+ signals represent the optical readout of AP activity in IHCs (Figure 1C). While individual APs could be detected by Ca2+ imaging (Figure 1C: left), bursts of APs resulted in an overall increase in the fluorescence level (Figure 1C: right) because fluorescence emission increased rapidly, but decayed with an average time constant of 300 ± 11 ms (n = 7 APs; Figure 1D), which is likely to reflect the dissociation constant (koff) of the high-affinity Ca2+ dye (Canepari and Mammano, 1999; Bortolozzi et al., 2008).

Intercellular Ca2+ waves in the GER propagate along different spatial directions

Using Ca2+ imaging we also found spontaneous propagation of intercellular Ca2+ waves in the GER, as previously reported (Tritsch et al., 2007; Schutz et al., 2010; Rodriguez et al., 2012; Xu et al., 2017; Mammano and Bortolozzi, 2018; Ceriani et al., 2019). Ca2+ waves occurred with a frequency of 3.46 ± 0.44/min in a field of view of 190 µm × 190 µm (10 recordings, 8 cochleae, 8 mice), and can be broadly classified as either radial or longitudinal (Figure 2 and Supplementary Video 2). The latter, which correspond to 14% of all waves (Figure 3A,B,C), propagated along the coiling axis of the cochlea across the NSCs that intercalate between IHCs with a speed of 7.6 ± 1.7 μm/s (n = 7 waves, 4 cochleae, 4 mice). Among the radial Ca2+ waves, i.e. those travelling in the direction orthogonal to the coiling axis (86%: Figure 3B,D,E), the majority (64%) travelled towards the bulk of the GER (5.7 ± 1.2 μm/s, n = 32 waves, 4 cochleae, 4 mice; Figure 3B,D) whereas only 22% spread towards the IHCs (5.3 ± 1.2 μm/s, n = 11 waves, 4 cochleae, 4 mice; Figure 3B,E).

AP activity in IHCs and Ca2+ wave propagation in the GER exhibit variable degrees of correlation

Ca2+ imaging revealed that IHCs fired Ca2+ APs (as reported optically) also in the complete absence of detectable Ca2+ activity in the GER (Figure 4A,B). Without Ca2+ waves in the GER (e.g. during time interval T1 in Figure 4B,C), the IHC-IHC average correlation coefficient (correlation index, c, see Materials and Methods) was not significantly different from 0 (c = 0.02, n = 10 recordings from 9 mice, P = 0.1, Student’s t-test, Figure 4D), indicating that IHCs generated APs independently of each other. IHC Ca2+ activity increased when Ca2+ waves were present in the GER (e.g. during time interval T2 in Figure 4B,C; see also Supplementary Video 3), leading to an increased probability of synchronized bursting among many hair cells. In these conditions, correlation index values deviated significantly from 0 for 68 out of the 111 Ca2+ wave events analyzed (10 recordings from 9 mice, P<0.05, Student’s t-test) and displayed a monotonic dependence with the area of the tissue invaded by the Ca2+ wave (Pearson’s coefficient ρ = 0.6, Figure 4D).

To confirm that AP activity in IHCs and Ca2+ wave propagation in the GER can occur independently of each other, we performed simultaneous recording of Ca2+ signals from GER NSCs and cell-attached recordings of APs from IHCs (Figure 5 and Supplementary Video 4). When bursts of IHC AP activity were correlated to Ca2+ transients in nearby NSCs (Figure 5A,B), their frequency increased significantly (2.8 ± 0.1 Hz, n = 82 bursts in 7 IHCs) compared to the condition when no correlation was observed (1.4 ± 0.1 Hz, n = 51 bursts in 7 IHCs, P < 0.001; Figure 5C). AP burst duration was also significantly higher when correlated to non-sensory cell activity (correlated: 11.0 ± 1.5 s; uncorrelated: 2.9 ± 0.3 s, P < 0.001, Figure 5D). In these conditions, the longitudinal and radial dimensions of the GER area showing significant correlation with AP activity of a given IHC were 310 ± 49 μm and 121 ± 12 μm, respectively (n = 7 cochleae; Figure 6). This quantitative analysis suggests that GER Ca2+ waves promote synchronization of IHC AP activity by variable amounts, depending on wave extension.

Consistent with the observation that a fraction of the Ca2+ waves appeared to depart from the IHC region and travelling towards the bulk of the GER (Figure 4 and Supplementary Video 5), we found that IHCs depolarization triggered Ca2+ signals in nearby NSCs, with a delay that was proportional to the distance from the stimulated IHC (3 recordings from 3, Figure 7; Supplementary Video 6). Therefore, there appears to be a reciprocal relationship between Ca2+ signals generated by IHCs and NSCs of the GER.

Transgenic mice expressing genetically encoded Ca2+ biosensors illuminate AP activity

To gain further insight into the mechanisms that govern spontaneous Ca2+ signaling in the developing cochlea, we used transgenic mice (see Materials and Methods) that expressed Ca2+ biosensors either in the whole sensory epithelium (GCaMP3;Emx2-Cre mice, Figure 8A and Supplementary Video 7) or selectively in hair cells (GCaMP3;Gfi1-Cre mice, Figure 8B and Supplementary Video 8, and GCaMP6f;Gfi1-Cre mice, Figure 8C and Supplementary Video 9). The higher contrast and signal-to-noise ratio afforded by cultures obtained from these mice, permitted us to partition IHC Ca2+ signals in two broad classes, namely low-amplitude (e.g. those corresponding to downward arrowheads in Figure 8D) and large-amplitude Ca2+ transients (e.g. downward arrows in Figure 8D). Whereas the IHC low-amplitude events were largely uncorrelated, the IHC large-amplitude events occurred only in the presence of Ca2+ waves in the GER and were correlated within a group of contiguous IHCs (Figure 9A). The two types of signals could be also discriminated pharmacologically. In prior work (Rodriguez et al., 2012) spontaneous Ca2+ signaling and Ca2+ wave propagation in the GER were reversibly reduced by the phospholipase C (PLC) inhibitor U73122 as well as by the inositol 1,4,5-trisphosphate receptor (IP3R) antagonist 2-aminoethoxydiphenyl borate (2-APB), and irreversibly suppressed by thapsigargin, a noncompetitive inhibitor of the Ca2+-ATPase (SERCA) that causes the complete and irreversible depletion of Ca2+ from the endoplasmic reticulum (ER) Ca2+ store. In this work, both Ca2+ waves in the GER and IHC synchronous large-amplitude Ca2+ transients were abrogated by P2Y and P2X receptor antagonists suramin (200 µM) and PPADS (100 µM), as well as by thapsigargin (10 µM), whereas ryanodine (50 µM) was not effective. However these drugs failed to suppress the desynchronized low-amplitude Ca2+ transients in IHCs (Figure 9B,C). In contrast, the latter were obliterated by nimodipine (50 µM), whereas Ca2+ waves in the GER were able to propagate in the presence of this L-type Ca2+ channels inhibitor (Supplementary Video 10). A summary of these results is presented in histogram form in Figure 9D. Together, the results in Figures 8 and 9 confirm that Ca2+ waves in the GER require the PIP2/PLC/IP3R signaling axis promoting Ca2+ release from ryanodine-insensitive intracellular Ca2+ stores (Rodriguez et al., 2012) and that synchronization of IHC activity by Ca2+ waves in the GER depends on extracellular ATP acting on IHCs (Johnson et al., 2011). They also support the tenet that IHC AP firing can occur independently of Ca2+ waves in the GER.

Patch clamp recordings reveal spontaneous APs in isolated IHCs

To confirm that Ca2+ APs in immature IHCs do not require Ca2+ waves in the GER, we performed whole-cell patch clamp recordings from mechanically isolated IHCs, which were obtained using a small suction pipette to remove the surrounding NSCs. This procedure did not compromise cell integrity, since these isolated IHCs showed normal outward K+ currents (Figure 10A: amplitude measured at 0 mV: 2.6 ± 0.2 nA, n = 3, P2) and a resting membrane potential (−62.0 ± 0.7 mV, n = 3) similar to that recorded from IHCs kept in situ (Marcotti et al., 2003a; Marcotti et al., 2003b). Importantly, isolated IHCs exhibited spontaneous APs (Figure 10B), indicating that this firing activity is an intrinsic property of immature IHCs that can be modulated by the spontaneous Ca2+ waves originating from the GER.

Figure 10.
Figure 10. Whole cell recordings from isolated IHCs

(A) Typical current responses from an isolated P2 IHCs recorded from the apical coil of the cochlea of wild-type mice. Outward currents were elicited by using depolarizing voltage steps (10 mV increments) from the holding potential of –84 mV to the various test potentials shown by some of the traces. (B) Spontaneous action potentials recorded from an isolated P2 apical IHC using whole-cell voltage clamp. IHCs were isolated by using a small pipette to remove the surrounding non-sensory cells.

DISCUSSION

Using a combination of Ca2+ imaging and cell-attached patch clamp recordings performed at body temperature, we have found that AP activity in mouse pre-hearing IHCs is intrinsically generated by the cells themselves. A stringent cross-correlation analysis has revealed that only the Ca2+ waves in the NSCs originating within specific distances from IHCs (∼300 µm along the coiling axis of the cochlea and ∼120 µm in the orthogonal, radial, direction) act as an extrinsic pathway to synchronize the intrinsic firing activity of IHCs. We also found that a large fraction of these Ca2+ waves originating in the proximity of the IHCs were able to propagate away from the sensory cells towards the bulk of the GER. IHCs depolarization also triggered Ca2+ signals in NSCs, which propagated towards the GER, indicating the presence of a bi-directional signaling within the immature organ of Corti. We also found that synchronization of IHC activity by Ca2+ waves in the GER depends on extracellular ATP directly acting on IHCs (Johnson et al., 2011). We argue that a combination of intrinsic activity and mutual influence between IHCs and supporting cells forms an intricate feedback mechanism to control the level of AP synchronization in IHCs and generate the patterned activity implicated in the refinement of the auditory pathway before the onset of hearing.

Nature of spontaneous activity in cochlear non-sensory cells

In the GER, spontaneous Ca2+ transients arise periodically, and propagate as Ca2+ waves as shown in Figures 2 to 5. Our results (Figures 8 and 9) support the notion that Ca2+ waves in the GER require functional ryanodine-insensitive intracellular Ca2+ stores, which are activated by extracellular ATP. Specifically, the binding of ATP to P2Y promotes the generation of diacylglycerol and IP3 from PLC-dependent hydrolysis of PIP2. Intracellular diffusion of IP3 and subsequent binding to IP3 receptors triggers Ca2+ release from the ER, increasing the cytosolic Ca2+ concentration to peak levels of ∼500 nM (Beltramello et al., 2005; Ceriani et al., 2016a). This elevated Ca2+ concentration has been shown to increase the open probability of connexin hemichannels expressed in NSCs (De Vuyst et al., 2006; Zhang et al., 2006; De Vuyst et al., 2009; Leybaert et al., 2017; Carrer et al., 2018; Hu et al., 2018), which favors the release of ATP from cytosol to extracellular milieu through hemichannels composed of Cx26 and Cx30 protomers (Anselmi et al., 2008; Majumder et al., 2010; Xu et al., 2017; Mammano, 2019). Purinergic signaling is terminated by ectonucleotidases (Housley et al., 2002; Vlajkovic et al., 2004) which degrade extracellular ATP (Zimmermann et al., 2012). Thus, ATP–dependent ATP–release enables the regenerative cell–to–cell propagation of Ca2+ signals across the network of cochlear non– sensory cells by exploiting a cascade of biochemical reactions governed by critical phenomena that control also the frequency of cytosolic Ca2+ oscillation (Ceriani et al., 2016a).

Nature of spontaneous activity in cochlear hair cells

Although cochlear hair cells are already visible at E14.5, and exhibit biophysical properties compatible with immature differentiating IHCs (Marcotti et al., 2003a), their maturation into fully functional sensory receptors only occurs at the onset of hearing (Kros et al., 1998).

During pre-hearing stages of development, both IHCs and OHCs are capable of eliciting Ca2+-dependent APs (IHCs: (Kros et al., 1998; Beutner and Moser, 2001; Marcotti et al., 2003b; Johnson et al., 2011); OHCs: (Ceriani et al., 2019). Calcium AP activity in apical coil IHCs occurs in bursts-like modality (Johnson et al., 2011; Eckrich et al., 2018). The present results, and a vast body of prior work, indicate that these APs are intrinsically generated by immature hair cells, since they are present in the absence of spontaneous Ca2+ waves in NSCs (IHCs, Johnson et al., 2017; Eckrich et al., 2018; Harrus et al., 2018; OHCs, Ceriani et al., 2019), and can be recorded from isolated IHCs (Figure 10). This spontaneous firing activity is possible because cochlear hair cells express L-type Cav1.3 voltage-gated Ca2+ channels (Platzer et al., 2000; Michna et al., 2003) that activate at about −70 mV (Zampini et al., 2010), which is more negative than their average resting membrane potential (about −65 mV) (Marcotti et al., 2003b). This intrinsic activity has been shown to be modulated by the cholinergic inhibitory medial olivocochlear fibers (Glowatzki and Fuchs, 2000), which form direct, but transient, synapses with immature IHCs (Simmons et al., 1996a; Simmons et al., 1996b). Cholinergic Ca2+ signals are controlled and compartmentalized by high levels of intracellular Ca2+ buffering and “subsynaptic” cisterns (Moglie et al., 2018). The activation of the efferent system causes immature IHCs to hyperpolarize, thereby reducing the frequency of spontaneous APs (Glowatzki and Fuchs, 2000; Marcotti et al., 2004; Johnson et al., 2011). In mice lacking a functional efferent innervation, both the maturation of the hair cell’s ribbon synapses (Johnson et al., 2013) and the refining of the immature tonotopic maps in the auditory brainstem nuclei (Clause et al., 2014) is impaired. IHC firing activity can also be modulated in the developing cochlea by the mechanoelectrical transducer channel, which is crucial for the maturation of the IHCs (Corns et al., 2018), and by ATP-induced intercellular Ca2+ waves from connexin extrajunctional hemichannels in the NSCs in the GER (Tritsch et al., 2007; Schutz et al., 2010; Rodriguez et al., 2012).

Despite the large variability in the direction of propagation, all Ca2+ waves reaching the IHC area produced an increased firing activity (long bursts: Figures 1,5; see also Eckrich et al., 2018), leading to synchronized firing between nearby IHCs (Figure 4). Several data indicate that ATP release from connexin hemichannels in NSCs, which express mainly Cx26 and Cx30, is able to affect IHC activity directly (Tritsch et al., 2007; Johnson et al., 2011), which is also supported by recent observations showing that the application of ATP is able to increase IHC firing prior to the induction of Ca2+ waves in the GER NSCs (Eckrich et al., 2018). An alternative mechanism is that ATP, by acting on purinergic auto-receptors expressed in the supporting cells surrounding the IHCs, leads to the opening of TMEM16A Ca2+-activated Cl- channels and the efflux of K+ and the depolarization of the sensory cells (Wang et al., 2015). However, a recent work has shown that synchronization of the activity of nearby IHCs was also observed in the absence of Ca2+ waves in cells of the GER (Eckrich et al., 2018), and suggested instead that it is the efflux of K+ from the IHCs during repetitive APs that depolarize neighbouring IHCs and thus coordinating their electrical activity. As mentioned above, we found that prolonged IHC depolarization, which is likely to results in elevation of [K+] in the confined extracellular space between IHCs and inner supporting cells (ISCs), triggered Ca2+ transients in NSCs (Figure 7).

Further implications for the observed Ca2+ signaling activity

Ca2+ waves are known to be accompanied by crenation of NSCs, an osmotic effect which determines the transient rupture of cell-cell contacts within Kölliker’s organ following the opening TMEM16A Ca2+-activated chloride channels expressed by these cells (Tritsch et al., 2007; Wang et al., 2015). These cellular process correlate with expression of apoptosis and autophagy markers in NSCs of the GER (Hou et al., 2019). Programmed cell death is crucial for animal development and Ca2+ signaling contributes to organogenesis, topological organization and orientation (Brodskiy et al., 2019; Fontana et al., 2019) by the interplay of apoptosis and autophagy (La Rovere et al., 2016; Giorgi et al., 2018). Therefore, we speculate that, besides modulating AP firing in IHCs, Ca2+ waves are likely to support the tightly regulated autophagic and apoptotic processes required for the development and formation of the mature cochlear sensory epithelium. Indirect support for this hypothesis is offered, for example, by the evidence that normal hair cell development is impaired in knockout mice for Cx26 and Cx30 (Johnson et al., 2017), which is followed by the degeneration of both hair cells and NSCs (Crispino et al., 2011). These Cx deficient mice were also shown to have increased levels of oxidative stress in the cochlea due to impairment of Nrf2/ARE signaling, accelerated age-related hearing loss (Fetoni et al., 2018). In multiple cell types, oxidative stress potentiates IP3–receptor 1 (IP3R1)–mediated Ca2+ release by oxidation of numerous cysteine residues (Joseph et al., 2018), and disturbed Ca2+ signaling has the potential to derail the course of autophagy and cell death (La Rovere et al., 2016).

Summarizing, it has been very effectively pointed out that “each Ca2+ wave is a specific and unique code that is indispensable for the transfer of important information based on its precise amplitude, frequency, timing, and duration” (Giorgi et al., 2018). The Ca2+ signaling described in this article sits at a crucial crossroad between development and its derailment, autophagy, apoptosis and premature aging of the mammalian auditory system.

Acknowledgements

This work was supported by Fondazione Telethon (grant GGP13114 to FM), the University of Padova (Progetto Strategico DYCENDI, prot. STPD11ALFE, to FM), The Wellcome Trust (grant 102892 to WM) and NIH intramural research funds (Z01-DC000002 to B.K.). FC was partially supported by a junior post-doctoral fellowship from the University of Padova (grant CPDR132235 to FM). SLJ is a Royal Society URF.

Footnotes

  • ↵* Joint first authors

  • Author Information: The authors declare that they have no competing financial interest.

REFERENCES

  1. ↵
    Abitbol JM, O’Donnell BL, Wakefield CB, Jewlal E, Kelly JJ, Barr K, Willmore KE, Allman BL, Penuela S (2019) Double deletion of Panx1 and Panx3 affects skin and bone but not hearing. J Mol Med (Berl) 97:723–736.
    OpenUrl
  2. ↵
    Afrashteh N, Inayat S, Mohsenvand M, Mohajerani MH (2017) Optical-flow analysis toolbox for characterization of spatiotemporal dynamics in mesoscale optical imaging of brain activity. Neuroimage 153:58–74.
    OpenUrl
  3. ↵
    Anselmi F, Hernandez VH, Crispino G, Seydel A, Ortolano S, Roper SD, Kessaris N, Richardson W, Rickheit G, Filippov MA, Monyer H, Mammano F (2008) ATP release through connexin hemichannels and gap junction transfer of second messengers propagate Ca2+ signals across the inner ear. Proc Natl Acad Sci U S A 105:18770–18775.
    OpenUrlAbstract/FREE Full Text
  4. ↵
    Beltramello M, Piazza V, Bukauskas FF, Pozzan T, Mammano F (2005) Impaired permeability to Ins(1,4,5)P3 in a mutant connexin underlies recessive hereditary deafness. Nat Cell Biol 7:63–69.
    OpenUrlCrossRefPubMedWeb of Science
  5. ↵
    Beutner D, Moser T (2001) The presynaptic function of mouse cochlear inner hair cells during development of hearing. J Neurosci 21:4593–4599.
    OpenUrlAbstract/FREE Full Text
  6. ↵
    Bootman MD, Rietdorf K, Collins T, Walker S, Sanderson M (2013) Ca2+-sensitive fluorescent dyes and intracellular Ca2+ imaging. Cold Spring Harb Protoc 2013:83–99.
    OpenUrlPubMed
  7. ↵
    Bortolozzi M, Lelli A, Mammano F (2008) Calcium microdomains at presynaptic active zones of vertebrate hair cells unmasked by stochastic deconvolution. Cell Calcium 44:158–168.
    OpenUrlCrossRefPubMedWeb of Science
  8. ↵
    Brodskiy PA, Wu Q, Soundarrajan DK, Huizar FJ, Chen J, Liang P, Narciso C, Levis MK, Arredondo-Walsh N, Chen DZ, Zartman JJ (2019) Decoding Calcium Signaling Dynamics during Drosophila Wing Disc Development. Biophys J 116:725–740.
    OpenUrl
  9. ↵
    Canepari M, Mammano F (1999) Imaging neuronal calcium fluorescence at high spatio-temporal resolution. J Neurosci Methods 87:1–11.
    OpenUrlCrossRefPubMedWeb of Science
  10. ↵
    Carrer A, Leparulo A, Crispino G, Ciubotaru CD, Marin O, Zonta F, Bortolozzi M (2018) Cx32 hemichannel opening by cytosolic Ca2+ is inhibited by the R220X mutation that causes Charcot-Marie-Tooth disease. Hum Mol Genet 27:80–94.
    OpenUrl
  11. ↵
    Ceriani F, Pozzan T, Mammano F (2016a) Critical role of ATP-induced ATP release for Ca2+ signaling in nonsensory cell networks of the developing cochlea. Proc Natl Acad Sci U S A 113:E7194–E7201.
    OpenUrlAbstract/FREE Full Text
  12. ↵
    Ceriani F, Ciubotaru CD, Bortolozzi M, Mammano F (2016b) Design and Construction of a Cost-Effective Spinning Disk System for Live Imaging of Inner Ear Tissue. Methods Mol Biol 1427:223–241.
    OpenUrl
  13. ↵
    Ceriani F, Hendry A, Jeng JY, Johnson SL, Stephani F, Olt J, Holley MC, Mammano F, Engel J, Kros CJ, Simmons DD, Marcotti W (2019) Coordinated calcium signalling in cochlear sensory and non-sensory cells refines afferent innervation of outer hair cells. EMBO J 38.
  14. ↵
    Clause A, Kim G, Sonntag M, Weisz CJ, Vetter DE, Rubsamen R, Kandler K (2014) The precise temporal pattern of prehearing spontaneous activity is necessary for tonotopic map refinement. Neuron 82:822–835.
    OpenUrlCrossRefPubMedWeb of Science
  15. ↵
    Corns LF, Johnson SL, Kros CJ, Marcotti W (2014) Calcium entry into stereocilia drives adaptation of the mechanoelectrical transducer current of mammalian cochlear hair cells. Proc Natl Acad Sci U S A 111:14918–14923.
    OpenUrlAbstract/FREE Full Text
  16. ↵
    Corns LF, Johnson SL, Roberts T, Ranatunga KM, Hendry A, Ceriani F, Safieddine S, Steel KP, Forge A, Petit C, Furness DN, Kros CJ, Marcotti W (2018) Mechanotransduction is required for establishing and maintaining mature inner hair cells and regulating efferent innervation. Nat Commun 9:4015.
    OpenUrl
  17. ↵
    Crispino G, Di Pasquale G, Scimemi P, Rodriguez L, Galindo Ramirez F, De Siati RD, Santarelli RM, Arslan E, Bortolozzi M, Chiorini JA, Mammano F (2011) BAAV mediated GJB2 gene transfer restores gap junction coupling in cochlear organotypic cultures from deaf Cx26Sox10Cre mice. PLoS One 6:e23279.
    OpenUrlCrossRefPubMed
  18. ↵
    De Vuyst E, Decrock E, Cabooter L, Dubyak GR, Naus CC, Evans WH, Leybaert L (2006) Intracellular calcium changes trigger connexin 32 hemichannel opening. Embo J 25:34–44.
    OpenUrlAbstract/FREE Full Text
  19. ↵
    De Vuyst E, Wang N, Decrock E, De Bock M, Vinken M, Van Moorhem M, Lai C, Culot M, Rogiers V, Cecchelli R, Naus CC, Evans WH, Leybaert L (2009) Ca(2+) regulation of connexin 43 hemichannels in C6 glioma and glial cells. Cell Calcium 46:176–187.
    OpenUrlCrossRefPubMedWeb of Science
  20. ↵
    Di Virgilio F, Steinberg TH, Silverstein SC (1989) Organic-anion transport inhibitors to facilitate measurement of cytosolic free Ca2+ with fura-2. Methods Cell Biol 31:453–462.
    OpenUrlCrossRefPubMedWeb of Science
  21. ↵
    Dulon D, Mollard P, Aran JM (1991) Extracellular ATP elevates cytosolic Ca2+ in cochlear inner hair cells. Neuroreport 2:69–72.
    OpenUrlPubMedWeb of Science
  22. ↵
    Eckrich T, Blum K, Milenkovic I, Engel J (2018) Fast Ca2+ Transients of Inner Hair Cells Arise Coupled and Uncoupled to Ca2+ Waves of Inner Supporting Cells in the Developing Mouse Cochlea. Frontiers in Molecular Neuroscience 11:264.
    OpenUrl
  23. ↵
    Fetoni AR, Zorzi V, Paciello F, Ziraldo G, Peres C, Raspa M, Scavizzi F, Salvatore AM, Crispino G, Tognola G, Gentile G, Spampinato AG, Cuccaro D, Guarnaccia M, Morello G, Van Camp G, Fransen E, Brumat M, Girotto G, Paludetti G, Gasparini P, Cavallaro S, Mammano F (2018) Cx26 partial loss causes accelerated presbycusis by redox imbalance and dysregulation of Nfr2 pathway. Redox Biol 19:301–317.
    OpenUrl
  24. ↵
    Fisher RA (1915) Frequency Distribution of the Values of the Correlation Coefficient in Samples from an Indefinitely Large Population. Biometrika 10:507–521.
    OpenUrlCrossRef
  25. ↵
    Fontana JM, Khodus GR, Unnersjo-Jess D, Blom H, Aperia A, Brismar H (2019) Spontaneous calcium activity in metanephric mesenchymal cells regulates branching morphogenesis in the embryonic kidney. FASEB J 33:4089–4096.
    OpenUrl
  26. ↵
    Forge A, Becker D, Casalotti S, Edwards J, Marziano N, Nevill G (2003) Gap junctions in the inner ear: comparison of distribution patterns in different vertebrates and assessement of connexin composition in mammals. J Comp Neurol 467:207–231.
    OpenUrlCrossRefPubMedWeb of Science
  27. ↵
    Giorgi C, Danese A, Missiroli S, Patergnani S, Pinton P (2018) Calcium Dynamics as a Machine for Decoding Signals. Trends Cell Biol 28:258–273.
    OpenUrl
  28. ↵
    Glowatzki E, Fuchs PA (2000) Cholinergic synaptic inhibition of inner hair cells in the neonatal mammalian cochlea. Science 288:2366–2368.
    OpenUrlAbstract/FREE Full Text
  29. ↵
    Harrus AG, Ceccato JC, Sendin G, Bourien J, Puel JL, Nouvian R (2018) Spiking Pattern of the Mouse Developing Inner Hair Cells Is Mostly Invariant Along the Tonotopic Axis. Front Cell Neurosci 12:407.
    OpenUrl
  30. ↵
    Hinojosa R (1977) A note on development of Corti’s organ. Acta Otolaryngol 84:238–251.
    OpenUrlCrossRefPubMed
  31. ↵
    Hou S, Chen J, Yang J (2019) Autophagy precedes apoptosis during degeneration of the Kolliker’s organ in the development of rat cochlea. Eur J Histochem 63.
  32. ↵
    Housley GD, Jagger DJ, Greenwood D, Raybould NP, Salih SG, Jarlebark LE, Vlajkovic SM, Kanjhan R, Nikolic P, Munoz DJ, Thorne PR (2002) Purinergic regulation of sound transduction and auditory neurotransmission. Audiol Neurootol 7:55–61.
    OpenUrlCrossRefPubMed
  33. ↵
    Hu Z, Riquelme MA, Wang B, Bugay V, Brenner R, Gu S, Jiang JX (2018) Cataract-associated Connexin 46 Mutation Alters Its Interaction with Calmodulin and Function of Hemichannels. J Biol Chem.
  34. ↵
    Johnson SL, Forge A, Knipper M, Munkner S, Marcotti W (2008) Tonotopic variation in the calcium dependence of neurotransmitter release and vesicle pool replenishment at mammalian auditory ribbon synapses. J Neurosci 28:7670–7678.
    OpenUrlAbstract/FREE Full Text
  35. ↵
    Johnson SL, Kennedy HJ, Holley MC, Fettiplace R, Marcotti W (2012) The resting transducer current drives spontaneous activity in prehearing Mammalian cochlear inner hair cells. J Neurosci 32:10479–10483.
    OpenUrlAbstract/FREE Full Text
  36. ↵
    Johnson SL, Wedemeyer C, Vetter DE, Adachi R, Holley MC, Elgoyhen AB, Marcotti W (2013) Cholinergic efferent synaptic transmission regulates the maturation of auditory hair cell ribbon synapses. Open Biol 3:130163.
    OpenUrlCrossRefPubMed
  37. ↵
    Johnson SL, Ceriani F, Houston O, Polishchuk R, Polishchuk E, Crispino G, Zorzi V, Mammano F, Marcotti W (2017) Connexin-Mediated Signaling in Nonsensory Cells Is Crucial for the Development of Sensory Inner Hair Cells in the Mouse Cochlea. J Neurosci 37:258–268.
    OpenUrlAbstract/FREE Full Text
  38. ↵
    Johnson SL, Eckrich T, Kuhn S, Zampini V, Franz C, Ranatunga KM, Roberts TP, Masetto S, Knipper M, Kros CJ, Marcotti W (2011) Position-dependent patterning of spontaneous action potentials in immature cochlear inner hair cells. Nat Neurosci 14:711–717.
    OpenUrlCrossRefPubMed
  39. ↵
    Joseph SK, Young MP, Alzayady K, Yule DI, Ali M, Booth DM, Hajnoczky G (2018) Redox regulation of type-I inositol trisphosphate receptors in intact mammalian cells. J Biol Chem 293:17464–17476.
    OpenUrlAbstract/FREE Full Text
  40. ↵
    Kelley MW (2007) Cellular commitment and differentiation in the organ of Corti. Int J Dev Biol 51:571–583.
    OpenUrlCrossRefPubMedWeb of Science
  41. ↵
    Kikuchi K, Hilding D (1965) The Development of the Organ of Corti in the Mouse. Acta Oto-Laryngologica 60:207–221.
    OpenUrlCrossRefPubMed
  42. ↵
    Kimura J, Suda Y, Kurokawa D, Hossain ZM, Nakamura M, Takahashi M, Hara A, Aizawa S (2005) Emx2 and Pax6 Function in Cooperation with Otx2 and Otx1 to Develop Caudal Forebrain Primordium That Includes Future Archipallium. The Journal of Neuroscience 25:5097.
    OpenUrlAbstract/FREE Full Text
  43. ↵
    Kros CJ, Ruppersberg JP, Rusch A (1998) Expression of a potassium current in inner hair cells during development of hearing in mice. Nature 394:281–284.
    OpenUrlCrossRefPubMedWeb of Science
  44. ↵
    La Rovere RM, Roest G, Bultynck G, Parys JB (2016) Intracellular Ca(2+) signaling and Ca(2+) microdomains in the control of cell survival, apoptosis and autophagy. Cell Calcium 60:74–87.
    OpenUrlCrossRef
  45. ↵
    Leybaert L, Lampe PD, Dhein S, Kwak BR, Ferdinandy P, Beyer EC, Laird DW, Naus CC, Green CR, Schulz R (2017) Connexins in Cardiovascular and Neurovascular Health and Disease: Pharmacological Implications. Pharmacol Rev 69:396–478.
    OpenUrlAbstract/FREE Full Text
  46. ↵
    Madisen L, Garner AR, Shimaoka D, Chuong AS, Klapoetke NC, Li L, van der Bourg A, Niino Y, Egolf L, Monetti C, Gu H, Mills M, Cheng A, Tasic B, Nguyen TN, Sunkin SM, Benucci A, Nagy A, Miyawaki A, Helmchen F, Empson RM, Knopfel T, Boyden ES, Reid RC, Carandini M, Zeng H (2015) Transgenic mice for intersectional targeting of neural sensors and effectors with high specificity and performance. Neuron 85:942–958.
    OpenUrlCrossRefPubMed
  47. ↵
    Majumder P, Crispino G, Rodriguez L, Ciubotaru CD, Anselmi F, Piazza V, Bortolozzi M, Mammano F (2010) ATP-mediated cell-cell signaling in the organ of Corti: the role of connexin channels. Purinergic Signal 6:167–187.
    OpenUrlCrossRefPubMedWeb of Science
  48. ↵
    Mammano F (2019) Inner Ear Connexin Channels: Roles in Development and Maintenance of Cochlear Function. Cold Spring Harb Perspect Med 9.
  49. ↵
    Mammano F, Bortolozzi M (2018) Ca(2+) signaling, apoptosis and autophagy in the developing cochlea: Milestones to hearing acquisition. Cell Calcium 70:117–126.
    OpenUrl
  50. ↵
    Marcotti W, Johnson SL, Holley MC, Kros CJ (2003a) Developmental changes in the expression of potassium currents of embryonic, neonatal and mature mouse inner hair cells. J Physiol 548:383–400.
    OpenUrlCrossRefPubMedWeb of Science
  51. ↵
    Marcotti W, Johnson SL, Rusch A, Kros CJ (2003b) Sodium and calcium currents shape action potentials in immature mouse inner hair cells. J Physiol 552:743–761.
    OpenUrlCrossRefPubMedWeb of Science
  52. ↵
    Marcotti W, Johnson SL, Kros CJ (2004) A transiently expressed SK current sustains and modulates action potential activity in immature mouse inner hair cells. J Physiol 560:691–708.
    OpenUrlCrossRefPubMedWeb of Science
  53. ↵
    Michna M, Knirsch M, Hoda JC, Muenkner S, Langer P, Platzer J, Striessnig J, Engel J (2003) Cav1.3 (alpha1D) Ca2+ currents in neonatal outer hair cells of mice. J Physiol 553:747–758.
    OpenUrlCrossRefPubMedWeb of Science
  54. ↵
    Mikaelian D, Ruben RJ (1965) Development of Hearing in the Normal Cba-J Mouse: Correlation of Physiological Observations with Behavioral Responses and with Cochlear Anatomy. Acta Oto-Laryngologica 59:451–461.
    OpenUrlCrossRef
  55. ↵
    Moglie MJ, Fuchs PA, Elgoyhen AB, Goutman JD (2018) Compartmentalization of antagonistic Ca(2+) signals in developing cochlear hair cells. Proc Natl Acad Sci U S A 115:E2095–E2104.
    OpenUrlAbstract/FREE Full Text
  56. ↵
    Ortolano S, Di Pasquale G, Crispino G, Anselmi F, Mammano F, Chiorini JA (2008) Coordinated control of connexin 26 and connexin 30 at the regulatory and functional level in the inner ear. Proc Natl Acad Sci U S A 105:18776–18781.
    OpenUrlAbstract/FREE Full Text
  57. ↵
    Platzer J, Engel J, Schrott-Fischer A, Stephan K, Bova S, Chen H, Zheng H, Striessnig J (2000) Congenital deafness and sinoatrial node dysfunction in mice lacking class D L-type Ca2+ channels. Cell 102:89–97.
    OpenUrlCrossRefPubMedWeb of Science
  58. ↵
    Rodriguez L, Simeonato E, Scimemi P, Anselmi F, Cali B, Crispino G, Ciubotaru CD, Bortolozzi M, Ramirez FG, Majumder P, Arslan E, De Camilli P, Pozzan T, Mammano F (2012) Reduced phosphatidylinositol 4,5-bisphosphate synthesis impairs inner ear Ca2+ signaling and high-frequency hearing acquisition. Proc Natl Acad Sci U S A 109:14013–14018.
    OpenUrlAbstract/FREE Full Text
  59. ↵
    Schutz M, Scimemi P, Majumder P, De Siati RD, Crispino G, Rodriguez L, Bortolozzi M, Santarelli R, Seydel A, Sonntag S, Ingham N, Steel KP, Willecke K, Mammano F (2010) The human deafness-associated connexin 30 T5M mutation causes mild hearing loss and reduces biochemical coupling among cochlear non-sensory cells in knock-in mice. Hum Mol Genet 19:4759–4773.
    OpenUrlCrossRefPubMedWeb of Science
  60. ↵
    Shnerson A, Pujol R (1981) Age-related changes in the C57BL/6J mouse cochlea. I. Physiological findings. Brain Res 254:65–75.
    OpenUrlCrossRefPubMed
  61. ↵
    Simmons DD, Mansdorf NB, Kim JH (1996a) Olivocochlear innervation of inner and outer hair cells during postnatal maturation: evidence for a waiting period. J Comp Neurol 370:551–562.
    OpenUrlCrossRefPubMedWeb of Science
  62. ↵
    Simmons DD, Moulding HD, Zee D (1996b) Olivocochlear innervation of inner and outer hair cells during postnatal maturation: an immunocytochemical study. Brain Res Dev Brain Res 95:213–226.
    OpenUrlCrossRefPubMed
  63. ↵
    Sugasawa M, Erostegui C, Blanchet C, Dulon D (1996) ATP activates non-selective cation channels and calcium release in inner hair cells of the guinea-pig cochlea. J Physiol 491 (Pt 3):707–718.
    OpenUrlPubMedWeb of Science
  64. ↵
    Teubner B, Michel V, Pesch J, Lautermann J, Cohen-Salmon M, Sohl G, Jahnke K, Winterhager E, Herberhold C, Hardelin JP, Petit C, Willecke K (2003) Connexin30 (Gjb6)-deficiency causes severe hearing impairment and lack of endocochlear potential. Hum Mol Genet 12:13–21.
    OpenUrlCrossRefPubMedWeb of Science
  65. ↵
    Tritsch NX, Yi E, Gale JE, Glowatzki E, Bergles DE (2007) The origin of spontaneous activity in the developing auditory system. Nature 450:50–55.
    OpenUrlCrossRefPubMedWeb of Science
  66. ↵
    Vlajkovic SM, Housley GD, Munoz DJ, Robson SC, Sevigny J, Wang CJ, Thorne PR (2004) Noise exposure induces up-regulation of ecto-nucleoside triphosphate diphosphohydrolases 1 and 2 in rat cochlea. Neuroscience 126:763–773.
    OpenUrlCrossRefPubMed
  67. ↵
    Wang HC, Lin CC, Cheung R, Zhang-Hooks Y, Agarwal A, Ellis-Davies G, Rock J, Bergles DE (2015) Spontaneous Activity of Cochlear Hair Cells Triggered by Fluid Secretion Mechanism in Adjacent Support Cells. Cell 163:1348–1359.
    OpenUrlCrossRefPubMed
  68. ↵
    1. Dallos P,
    2. Popper, A.,
    3. Fay, R.
    Wangemann P, Schacht, J. (1996) Homeostatic mechanism in the cochlea. In: The Cochlea (Dallos P, Popper, A., Fay, R., ed), pp 130–185. New York: Springer-Verlag.
  69. ↵
    Xu L, Carrer A, Zonta F, Qu Z, Ma P, Li S, Ceriani F, Buratto D, Crispino G, Zorzi V, Ziraldo G, Bruno F, Nardin C, Peres C, Mazzarda F, Salvatore AM, Raspa M, Scavizzi F, Chu Y, Xie S, Yang X, Liao J, Liu X, Wang W, Wang S, Yang G, Lerner RA, Mammano F (2017) Design and Characterization of a Human Monoclonal Antibody that Modulates Mutant Connexin 26 Hemichannels Implicated in Deafness and Skin Disorders. Front Mol Neurosci 10:298.
    OpenUrl
  70. ↵
    Yang H, Gan J, Xie X, Deng M, Feng L, Chen X, Gao Z, Gan L (2010) Gfi1-Cre knock-in mouse line: A tool for inner ear hair cell-specific gene deletion. genesis 48:400–406.
    OpenUrlCrossRefPubMedWeb of Science
  71. ↵
    Zampini V, Johnson SL, Franz C, Lawrence ND, Munkner S, Engel J, Knipper M, Magistretti J, Masetto S, Marcotti W (2010) Elementary properties of CaV1.3 Ca(2+) channels expressed in mouse cochlear inner hair cells. J Physiol 588:187–199.
    OpenUrlCrossRefPubMed
  72. ↵
    Zhang X, Zou T, Liu Y, Qi Y (2006) The gating effect of calmodulin and calcium on the connexin50 hemichannel. Biol Chem 387:595–601.
    OpenUrlPubMed
  73. ↵
    Zhou P, Resendez SL, Rodriguez-Romaguera J, Jimenez JC, Neufeld SQ, Giovannucci A, Friedrich J, Pnevmatikakis EA, Stuber GD, Hen R, Kheirbek MA, Sabatini BL, Kass RE, Paninski L (2018) Efficient and accurate extraction of in vivo calcium signals from microendoscopic video data. eLife 7:e28728.
    OpenUrlCrossRefPubMed
  74. ↵
    Zimmermann H, Zebisch M, Strater N (2012) Cellular function and molecular structure of ectonucleotidases. Purinergic Signal 8:437–502.
    OpenUrlCrossRefPubMedWeb of Science
  75. ↵
    Zorzi V, Paciello F, Ziraldo G, Peres C, Mazzarda F, Nardin C, Pasquini M, Chiani F, Raspa M, Scavizzi F, Carrer A, Crispino G, Ciubotaru CD, Monyer H, Fetoni AR A MS, Mammano F (2017) Mouse Panx1 Is Dispensable for Hearing Acquisition and Auditory Function. Front Mol Neurosci 10:379.
    OpenUrl
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Posted August 10, 2019.
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Dynamic coupling of cochlear inner hair cell intrinsic Ca2+ action potentials to Ca2+ signaling of non-sensory cells
Federico Ceriani, Stuart L. Johnson, Miloslav Sedlacek, Aenea Hendry, Bechara Kachar, Walter Marcotti, Fabio Mammano
bioRxiv 731851; doi: https://doi.org/10.1101/731851
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