Abstract
Voltage-gated calcium (Cav1.3) channels in mammalian inner hair cells (IHCs) open in response to sound and the resulting Ca2+ entry triggers the release of the neurotransmitter glutamate onto afferent terminals. At low to mid sound frequencies cell depolarization follows the sound sinusoid and pulses of transmitter release from the hair cell generate excitatory postsynaptic currents (EPSCs) in the afferent fiber that translate into a phase-locked pattern of action potential activity. The present article summarizes our current understanding on the elementary properties of single IHC Ca2+ channels, and how these could have functional implications for certain, poorly understood, features of synaptic transmission at auditory hair cell ribbon synapses.
Introduction
The mammalian auditory system has evolved specialized structures and cellular mechanisms that allow sound information to be relayed to the brain with unparalleled temporal precision. Our ability to localize sound sources in the environment depends on the preservation of timing accuracy along the auditory pathway. Low-frequency sounds are localized by specialized cells in the brainstem that compare the temporal delay between the phase-locked activity originating from the two ears, which can be as small as ten microseconds (Köppl, ; Carr and Macleod, ). The localization of high frequency sounds relies more on the detection of intensity differences between the outputs of the two ears, but the timing information obtained from the beginning and end of the sound envelope also has an important role (Moore, 1991; McAlpine, 2005). The intricate cellular mechanisms responsible for such exquisite temporal performance are still not well understood.
The initial step in the conversion of sound into an electrical signal takes place in the inner hair cells (IHCs), the primary sensory receptors of the cochlea, whereby sound-induced deflection of the hair bundle gates mechano-electrical transducer (MET) channels allowing the depolarizing flow of K+ ions into the cell. The interplay of the transducer current with the cells basolateral membrane currents generates the characteristic IHC receptor potential (Russell and Sellick, 1978), the size of which is graded to sound level. A fraction of MET channels are open at rest (Johnson et al., ), resulting in a tonic inflow of K+ which depolarizes the IHC in vivo. The in vivo resting membrane potential (Vm) activates a proportion of voltage-gated Ca2+ channels that is thought to drive the tonic release of glutamate onto afferent terminals (Glowatzki and Fuchs, ). The resulting AMPA-receptor-mediated post-synaptic depolarization is converted into a resting discharge of action potentials in the afferent fiber that is referred to as its spontaneous rate (Liberman, 1978). Upon sound stimulation, a greater proportion of MET channels are opened, which increases IHC depolarization and consequently Ca2+ influx/transmitter release. Any given IHC contacts numerous afferent nerve terminals, which extend from cochlear ganglion cells. IHCs provide the sole synaptic input to those neurons. Moreover, each IHC contacts a given ganglion cell through a single synaptic site; thus, all the information the hair cell has to transmit to the neuron must be funneled through that one synaptic site (Trussell, 2002). IHCs’ synaptic sites contain a special structure called the “ribbon”, which is covered with synaptic vesicles (von Gersdorff, 2001). Ribbons are thought to ensure a continuous supply of vesicles to the plasma membrane for exocytosis during endless ongoing stimulation (Fuchs, ). Moreover, at the presynaptic side of each ribbon synapse a pool of 16–30 ready-to-release docked vesicles can be typically observed (Khimich et al., ), which might account for the multivesicular release events recorded postsynaptically (Glowatzki and Fuchs, ). One could expect that increasing IHC depolarization will result in an increase of the amplitude and frequency of these multivesicular events. Instead, large excitatory post-synaptic current (EPSCs) can be recorded at rest, the frequency, but not amplitude, of which increases with IHC depolarization (Glowatzki and Fuchs, ; Goutman and Glowatzki, ).
Also still largely unexplained is the transduction system’s ability to phase-lock the afferent spiking to a particular time point (phase) of the low-to-mid-frequency sinusoidal sound wave independent of its intensity (Rose et al., 1967; Fuchs, ; Goutman, ). Indeed, increasingly larger receptor potentials, driven by increasingly louder sounds, should cause more Ca2+ influx and increasingly faster vesicular fusion (Fuchs, ).
In this article we focus on the elementary properties of IHC CaV1.3Ca2+ channels, which represent 90% of IHC Ca2+ channels (Platzer et al., 2000), and how they could underlie some of the still poorly understood characteristics of synaptic transmission at individual IHC ribbon synapses.
Results and Discussion
Ca2+ Channel Number and Open Probability
The total number of Ca2+ channels in a single IHC has been estimated in two ways: (1) using non-stationary fluctuation analysis of macroscopic (whole-cell) Ca2+ tail currents (Brandt et al., ; Vincent et al., 2014; Wong et al., 2014); and (2) by comparing the macroscopic (whole-cell) and elementary (cell-attached) Ca2+ current amplitudes (Zampini et al., 2010, 2013, 2014). The former uses the variability in size and shape of repeated deactivating Ca2+ tail currents (upon repolarization from a voltage step that activates the maximal macroscopic current) to estimate the channel number, single channel current and open probability (Po). The latter is a direct measure of elementary Ca2+ current (iCa) size and Po that is used to work out the number of channels from the size of the macroscopic Ca2+ current (ICa). The number of Ca2+ channels per IHC estimated from fluctuation analysis is about 1, 800 (Brandt et al., ; Vincent et al., 2014; Wong et al., 2014). In cell-attached recordings, Po was measured over long-lasting (500 ms) depolarizing voltage steps, in order to collect a large number of openings for reliable analysis. However, Ca2+ channels clearly underwent inactivation during these long pulses, as indicated by the shape of the ensemble-average currents (Zampini et al., 2013, 2014). If single channel analysis was limited to the initial 40 ms of the sweeps, Po (at about –20 mV) increased from 0.024 to 0.06 in middle-turn IHCs (Zampini et al., 2014) and from 0.21 (Zampini et al., 2013) to 0.51 in basal-turn IHCs (data re-analyzed for the present study).1 The resulting total number of Ca2+ channels would be 6, 400 in adult middle turn IHCs and 1, 152 in adult basal turn IHCs. For basal-turn IHCs, from which we have collected most data, an average of 1, 152 Ca2+ channels per IHC would equate to 74 channels per synapse and 5 channels per vesicle (Figure 1), given that there are 14 ribbon synapses per cell (Zampini et al., 2013) and 10% of Ca2+ channels are believed to be extrasynaptic (Meyer et al., 2009). This is consistent with the model proposed by Wong et al. (2014) for apical-coil mouse IHCs where there are estimated to be up to 90 Ca2+ channels per release site.
Figure 1
Ca2+ Channels and the Nanodomain
In a presynaptic nanodomain coupling of Ca2+ inflow—synaptic vesicle release (Stanley, 1993; Fedchyshyn and Wang, ), mathematical modeling predicts that a single Ca2+ channel may control vesicle release at each docking site (Weber et al., 2010). On the other hand, the opening of several Ca2+ channels may be necessary for the fusion of more distant vesicles at other synapses (microdomain; Borst and Sakmann, ). In IHCs, the linear Ca2+ dependence of exocytosis (Brandt et al., ; Johnson et al., , ; Goutman and Glowatzki, ) has been explained using a nanodomain model for the coupling between Ca2+ channels and synaptic vesicles. In such a model, the Ca2+ sensor for vesicle fusion is located within a radius of tens of nanometers from the Ca2+ channel (Moser et al., 2006), as found in the squid giant synapse (Neher, 1998; Augustine, ; Oheim et al., 2006). The assumption is that Ca2+ influx through a single channel is sufficient to activate release of a nearby vesicle. With depolarization, the increase in Ca2+ channel Po saturates the Ca2+ sensor, and therefore the postsynaptic response grows in linear proportion to the presynaptic Ca2+ current as additional Ca2+ channel openings bring with them their own “unit” of vesicular release. More direct evidence for the nanodomain coupling between Ca2+ channels and vesicle release sites in IHCs has come from the fact that the rapidly binding Ca2+ chelator BAPTA had a more prominent inhibitory effect on exocytosis than the more slowly acting EGTA (Moser and Beutner, 2000). The prediction is in fact that only the fast Ca2+ binding kinetics of BAPTA, but not the slower binding to EGTA, would be able to interrupt the action of Ca2+ in a nanodomain, as shown for the squid giant synapse (Adler et al., ; Augustine et al., ). However, Goutman and Glowatzki () found that different concentrations of EGTA were able to slow the onset and rise time of the fast component of release at the hair cell afferent synapse, concluding that the Ca2+ sensor (likely to be on the vesicle) is approximately 23 nm from the Ca2+ channel. Because of the high affinity of the Ca2+ sensor (Beutner et al., ), one or few Ca2+ channel openings might still be sufficient for activating release, reconciling the effect of EGTA with a nanodomain model. Although the molecular identity of the Ca2+ sensor remains uncertain (Safieddine and Wenthold, 1999; Roux et al., 2006; Beurg et al., ; Johnson et al., ; Pangrsic et al., 2010), its binding to Ca2+ is highly cooperative, seemingly requiring the binding of five calcium ions to trigger release (Beutner et al., ). Vesicular release becomes more sensitive to Ca2+ inflow during IHC maturation, showing a more classical high-order dependence on Ca2+-current (ICa) amplitude until the onset of hearing at around post-natal day 12, whereupon the release of synaptic vesicles becomes linearly dependent on ICa amplitude, as described above (Johnson et al., , ). Some authors have hypothesized that linearization might depend on a change in the Ca2+-sensor properties leading to lowered Ca2+-binding cooperativity (Murphy et al., 2004; Thoreson et al., 2004; Johnson et al., , ; Dulon et al., ). Heil and Neubauer () have shown that, in principle, a linear dependence of synaptic release on Ca2+ influx, as that observed in adult hair cells, can emerge if different release sites, each one of which endowed with the same, supralinear Ca2+ sensitivity, are differently exposed to Ca2+ entering through voltage-gated Ca2+ channels. To fit real data, 75% to 90% of release sites were required to be exposed to 20- to 200-fold lower Ca2+ concentrations than those most effectively exposed to Ca2+ inflow. This would imply that in adult IHCs most releasable vesicles are under the control of Ca2+ microdomains (rather than nanodomains), or that an even looser spatial relation exists between them and voltage-gated Ca2+ channels. Until this is not demonstrated, such interpretation can be regarded as an interesting theoretical possibility. Morphologically, maturation-dependent linearization of vesicular release on ICa amplitude is accompanied by a change in the IHC active zone/postsynaptic density complexes that are initially multiple, small and spot-like and then become large single structures. There is also a topographical re-arrangement of Ca2+ channels, which matches that of the active zones: Ca2+ channels are initially located in several smaller, round clusters and then form a larger stripe-like cluster (Wong et al., 2014). Indeed, in the absence of Eps8, which plays a crucial role in the physiological maturation of mammalian cochlear IHCs, the developmental linearization of the exocytotic Ca2+ sensitivity in IHCs does not occur (Zampini et al., 2011).
The nanodomain interaction between the active Ca2+ channel and the Ca2+ sensor (Figure 1) seems necessary to ensure that Ca2+ provided by one or a few Ca2+ channels is sufficient to trigger vesicle release with minimal delay before it diffuses away or is buffered. However, the nanodomain scenario does not necessarily mean that any Ca2+-channel opening, however brief, will be sufficient to saturate the Ca2+ sensor and trigger vesicle release. The idea that the Ca2+ sensor is easily saturated by single Ca2+ channel openings implies that, given the channel’s mean open time (τ), the fraction of channel openings long enough to saturate the Ca2+ sensor will be dominant over the fraction of shorter, non-saturating, openings. For instance, if a channel open duration equals to one tenth of τ (i.e., 1.65 ms at –20 mV; Zampini et al., 2013) is sufficient to saturate the Ca2+ sensor, then ~90% of the openings will be long enough to bring about the same result. This would facilitate the phase-locking of vesicle release to sound frequencies of a few kHz (Palmer and Russell, 1986) where it would need to be triggered by depolarizing stimuli as short as the positive-going phase of the stimulus (a few hundreds microseconds) whilst maintaining a constant phase relationship (Pickles, 1996; Rossing, 2007). The sub-ms activation and deactivation kinetics of IHC Ca2+ channels (first channel openings are estimated to occur with a delay of about 50 μs in physiological conditions; Zampini et al., 2013, 2014), would be suitably rapid to encode sound onset and support phase-locking.
Properties of EPSCs Generated by IHC Synapse Activation
Patch-clamp recordings from single nerve terminals contacting rat IHCs have shown that various types of EPSCs are evoked by IHC depolarization, from miniature EPSCs (mEPSCs) to large multi- or monophasic events seemingly resulting from the fusion of up to 20 vesicles (Glowatzki and Fuchs, ). The most abundant events (>70%), however, were large monophasic EPSCs (M-EPSCs), corresponding to the size of 3–6 summated mEPSCs (Glowatzki and Fuchs, ; Goutman and Glowatzki, ). M-EPSCs have also been observed in lower vertebrates, and presumed to result from the simultaneous release of multiple vesicles (Keen and Hudspeth, ; Suryanarayanan and Slaughter, 2006; Li et al., ; Schnee et al., 2013). Important for the following discussion, it has recently been suggested that M-EPSCs could underlie accurate phase-locking of spikes in the auditory fibers (Goutman, ; Li et al., ). In this section we attempt to reconcile the features of EPSCs with the properties of the single IHC Ca2+ channels.
The frequency of M-EPSCs during a step depolarization of IHCs increases in proportion to the stimulus amplitude, but at all voltages these large events appear to dominate over the lower-amplitude or less synchronous events. In immature rat IHCs, M-EPSC frequency was 2 Hz at –50 mV and 20 Hz at –20 mV (Goutman and Glowatzki, ) and seemed to be generally higher in more adult rats (Grant et al., ).
Under the assumption that mEPSCs are due to the release of single neurotransmitter quanta, and therefore correspond to the full fusion of single vesicles, the fact that M-EPSCs are the dominant postsynaptic events during sustained IHC depolarization suggests there is an intrinsic mechanism devoted to maximizing the release synchrony of a relatively homogeneous number of vesicles at IHC ribbon synapses. So far three models have been proposed for such a mechanism: (1) the ribbon itself, or proteins associated with the ribbon, facilitate the coordinated fusion of multiple vesicles docked at the active zone (Glowatzki and Fuchs, ; Singer et al., 2004); (2) the Ca2+ nanodomain around an open Ca2+ channel drives the simultaneous release of multiple vesicles (Jarsky et al., ; Graydon et al., ); and (3) multiple vesicles fuse together prior to fusing with the IHC membrane (termed compound fusion) (Matthews and Sterling, 2008). More recently, it has been proposed that the event corresponding to the full fusion of a single vesicle is in fact the M-EPSC, which would therefore represent a big-size elementary event, whereas the lower-amplitude EPSCs would result from incomplete or transitory fusion events, and multiphasic EPSCs from the flickering of the fusion pore between open and closed states (Chapochnikov et al., ). In the case of the incomplete or flickering fusion events, only small amounts of neurotransmitter would be released for every opening of the fusion pore, thus producing submaximal activation of postsynaptic receptors. Uniquantal release would also be consistent with the high rates of sound-driven spikes in spiral ganglion neurons (up to about Hz; Taberner and Liberman, 2005) given a maximal presynaptic release rate of about 700 Hz (Pangrsic et al., 2010)—see Figure 1 in Chapochnikov et al. ().
In a nanodomain scenario, hypotheses 2 and 3, as well as the model by Chapochnikov et al. (), would all be compatible with an M-EPSC being triggered by the opening of a single Ca2+ channel. In the case of hypothesis 1, the simultaneous opening of multiple Ca2+ channels, each associated with a different vesicle, could be required to activate the molecular machinery responsible for the coordinated, synchronous release of the same vesicle subset. It is unlikely, however, that multiple Ca2+ channel openings summate to produce M-EPSCs, given that M-EPSCs of similar amplitude are also observed, although at a much lower frequency, when the IHC is at rest, a membrane potential at which the probability of two or more Ca2+ channels being simultaneously open is negligible (Figure 1). Consistent with this hypothesis, EPSC size and shape heterogeneity persists when release probability is reduced by abolition of IHC Ca2+ influx (Chapochnikov et al., ), whereas synchronized M-EPSCs would be expected to become less represented in lower extracellular Ca2+.
Burst Openings of CaV1.3 Channels May Improve the Reliability of Synaptic Transmission in IHCs
Single-channel studies have revealed an interesting feature of CaV1.3 channels. We found that these channels are generally reluctant to open, but when they do, they open in bursts and maintain a very high open probability for a substantial amount of time (Zampini et al., 2010, 2013, 2014). In our recordings, a given Ca2+ channel could remain closed for several consecutive 500 ms depolarizing sweeps, and then suddenly shift to a bursting mode in which prolonged sequences of openings interrupted by brief closings produced periods of activity with a Po close to 1. Therefore, the majority of Ca2+ influx occurs via the bursting activity of Ca2+ channels, and is otherwise (i.e., outside bursts) negligible. Early studies on CaV1.2 channels also showed different modes of gating (Hess et al., ; Nowycky et al., 1985) which were called mode 0 (closed), 1 (brief and rare openings) and 2 (unusually long openings), and it was suggested that the exit from mode 0 depended on the metabolic state of the cell (Nowycky et al., 1985; Kamp and Hell, ; Carabelli et al., ). Mode 2 is favored by BayK 8644 (Hess et al., ; Nowycky et al., 1985; Ceña et al., ). In our experiments BayK 8644 was normally added to the pipette solution to increase Ca2+-channel activity, but mode 2 was also observed in the absence of BayK 8644 (Zampini et al., 2010).
We also found that, with depolarization, single Ca2+ channel kinetics mainly differed for the increase in importance of the shortest mean closed time, while mean open and closed time constants were relatively unaffected by membrane voltage (Zampini et al., 2013). Therefore, it appears that depolarization mainly favors the passage of the channel from a reluctant-to-open to a willing-to-open state. Once it opens, the Ca2+ channel open probability is then dominated by the burst modality of gating. This gating behavior suggests that at a given membrane potential the majority of Ca2+ channels are almost inactive (in modes 0 and 1), with the few channels opening in bursts (mode 2) underlying the majority of the macroscopic current recorded in whole-cell.2 Depolarization increases the chance that additional Ca2+ channels enter mode 2, accounting for the increase in the macroscopic current.
The likelihood that the majority of Ca2+ entry occurs during the burst opening of Ca2+ channels would have important implications as far as signal transmission at IHC afferent synapses is concerned. As discussed above, various lines of evidence suggest that IHC Ca2+ channels and release sites are within the spatial range of nanodomains, such that the opening of one channel might be sufficient to saturate the Ca2+ sensor and trigger vesicle release. One could hypothesize that, under these conditions, the most effective modality for Ca2+ channel opening in terms of vesicle release is burst opening. However, it is unlikely that the prolonged entry of Ca2+ during a burst is the necessary factor for vesicle release, since depolarizations of only a few hundred microseconds must be sufficient to trigger a release event during mid-frequency sound stimulation (see above).
It is more likely that a predominance of burst openings would improve the reliability of vesicle release. Let us assume, for example, that five Ca2+ channels are associated with a release-ready vesicle (see calculations above), with and average Po across all 5 channel of 0.2 (Figure 2A). This average Po could result from every one of the 5 channels having a Po of 0.2; or it could result from 4 out of 5 channels opening with a Po of 0.05, and one channel having a Po of 0.8 (corresponding to a burst) (Figure 2B). In the former scenario, the probability of no channels opening would be (1–0.2)5 = 0.33, whereas in the latter it would be (1–0.05)4·(1–0.8) = 0.16. In this example, a single bursting channel, even when the group of channels shows the same average Po as the non-bursting channels, would increase the probability of at least one Ca2+ channel being open at each active zone, from 0.67 to 0.84, which would increase the overall reliability of vesicle release.
Figure 2
Ca2+ Channel Properties and Phase-Locked Exocytosis
Afferent fibers innervating apical- and middle-turn cochlear IHCs show phase-locked spiking activity to sound frequencies up to a few kHz, independent of stimulus intensity (Figure 3A; Rose et al., 1967). The independence of phase-locking on intensity is hard to reconcile with either the Ca2+ microdomain or nanodomain control of IHC exocytosis. In a microdomain, Ca2+ influx through several Ca2+ channels at a presynaptic site would resemble the macroscopic ICa. Since ICa amplitude and activation speed increase with depolarization (Figure 3B), it is expected that neurotransmitter release will occur sooner the more intense the stimulus. In other words, increasing stimuli should produce progressively more phase-advanced afferent responses. A decrease in synaptic delay with increasing depolarization has been seen in rat IHCs (Goutman, ; see also Li et al., for frog auditory papilla hair cells). In a nanodomain, on the other hand, the latency-to-first Ca2+ channel opening decreases significantly with depolarization (Figure 3B). Therefore, either in a micro- or a nanodomain, depolarization would shorten the delay for Ca2+-dependent exocytosis and modify the phase of the response, interfering with phase-locking to that particular sound frequency.
Figure 3
A mechanism by which the accuracy of afferent phase-locking could be preserved independent of sound intensity has been proposed, involving the balance between short-term facilitation and depression of transmitter release at the hair cell ribbon synapse (Cho et al., ; Goutman, ). In this hypothesis, Ca2+ channel facilitation that occurs at voltages close to the resting membrane potential is compensated by synaptic vesicle depletion during prolonged trains of activity, producing a constant synaptic delay despite varying stimulus intensity (Goutman, ). However, a phase-advance should still be observed for the first cycles of the response before vesicle depletion occurs, whereas the first latencies (latency of the responses to first cycles) showed the same phase for all events (Goutman, ). This model, moreover, would imply that the afferent response to the first cycle/s of the sound wave would occur at different times depending on the sound level.
The properties of single Ca2+ channel currents could underlie the preservation of phase-locked transmission in a nanodomain in two possible ways. In the first scenario, as the IHC depolarizes, the amplitude of iCa decreases due to the reduction in driving force for Ca2+ entry (Figure 3B; Zampini et al., 2013). This would counteract the more rapid channel opening, such that the delay to Ca2+ sensor saturation for exocytosis may be comparable at different stimulus levels. This mechanism would allow the preservation of a constant phase relationship to changing sound intensity (Figure 4A). In a second scenario, a constant phase relation could be maintained by the effect of IHC repolarization on iCa. During the repolarizing phase of a rapid cyclic stimulus, the large increase in driving force for Ca2+ would increase the amplitude of the current flowing through an already open Ca2+ channel. If repolarization is sufficiently fast, the amplitude of the elementary Ca2+ current would quickly rise to levels high enough to promptly saturate the Ca2+ sensor. These “saturation events” will cluster in a limited time window during the repolarizing phase, regardless of the amplitude of the foregoing depolarization, as long as it has opened the Ca2+ channel. During the macroscopic Ca2+ “tail” currents elicited by fast repolarization, the amplitude of elementary currents would be maximized with minimal jitter (Figure 3B). Their duration would also be short, since channel deactivation is faster than activation, which would be favorable for phase-locking towards the upper sound frequency limit (Figure 4B). Recent studies have shown that when IHCs are stimulated with a voltage sinusoid to mimic sound, the largest M-EPSCs occurred most frequently during the repolarizing rather than the depolarizing phase (see e.g., Figure 3 in Goutman, ; Figure 5 in Li et al., ), even when the synaptic delay (0.7–0.8 ms; Palmer and Russell, 1986) is taken into account. During high-frequency stimulation, the maximal speed of macroscopic Ca2+ current development occurs during the early repolarizing phase of the cycle (Figure 5 in Li et al., ). Tail Ca2+ currents have been shown to elicit time-locked M-EPSCs (Goutman, ). Finally, M-EPSCs elicited by depolarizing voltage steps delivered to rat IHCs (Goutman, ) and frog auditory hair cells (Graydon et al., ) appear better phase-locked during the Ca2+ tail current upon repolarization rather than to the peak ICa. In the amphibian papilla, in which each afferent fiber receives input from several synaptic ribbons, the faster, less variable tail Ca2+ currents would seem better suited for triggering synchronous vesicle fusion than the stochastic opening of Ca2+ channels at different presynaptic sites. Therefore, in this second scenario, although IHC depolarization is necessary to open Ca2+ channels, subsequent IHC repolarization appears optimally suited for synchronizing post-synaptic activity with sound frequencies around the phase-locking limit.
Figure 4
In conclusion, it is possible that the elementary properties of IHC Ca2+ channels underlie several as yet unexplained features of the afferent response. The sub-ms first latency would ensure that at least some Ca2+ channels open with very short delay, allowing even relatively high frequency stimuli to be followed. The bursting behavior of Ca2+ channels, on the other hand, would increase the reliability of signal transmission. Finally, in a nanodomain where vesicle fusion is controlled by a single Ca2+ channel, the elementary current amplitude and opening latency could balance each other to produce constant phase-locking of the afferent response despite variations in sound intensity. The elementary tail currents would provide a rapid and large Ca2+ influx at the highest sound frequencies possible.
Author and Contributors
JM, PS, SLJ, and SM substantially contributed to the conception or design of the work, analysis and/or interpretation of data, drafting of the text and /or figures, revision, final approval of the version to be published and agree to be accountable for all aspects of the work in ensuring that questions related to the accuracy or integrity of any part of the work are appropriately investigated and resolved.
Statements
Funding
Acknowledgments
This work has been supported by Fondazione Cariplo, grant n° 2011-0596, to SM. SLJ is a Royal Society University Research Fellow.
Conflict of interest
The authors declare that the research was conducted in the absence of any commercial or financial relationships that could be construed as a potential conflict of interest.
Footnotes
1.^These values have been obtained in the presence of 5-μM BayK 8644, which stabilizes CaV1-channel openings and increases their Po. In the absence of BayK 8644, Po was approximately two-fold lower. Since, however, both whole-cell and cell-attached recordings were obtained in the presence of BayK 8644, the estimated number of Ca channel would not be invalidated. BayK 8644 is also routinely used in fluctuation-analysis studies to increase Po, which is favorable for estimating the channel number. Under such conditions, a maximal Po of ~0.8 has been estimated (Brandt et al., ; Vincent et al., 2014; Wong et al., 2014).
2.^Assuming that the same channel activity patterns also occur during whole-cell recording, the proportion of channels opening according to the high-Po, burst mode would conceivably dominate the macroscopic Ca currents, including tail currents. Therefore, only the subset of channels operating in the high-Po mode would be considered when fluctuation analysis is carried out.
References
1
AdlerE. M.AugustineG. J.DuffyS. N.CharltonM. P. (1991). Alien intracellular calcium chelators attenuate neurotransmitter release at the squid giant synapse. J. Neurosci.11, 1496–1507.
2
AugustineG. J. (2001). How does calcium trigger neurotransmitter release?Curr. Opin. Neurobiol.11, 320–326. 10.1016/s0959-4388(00)00214-2
3
AugustineG. J.SantamariaF.TanakaK. (2003). Local calcium signaling in neurons. Neuron40, 331–346. 10.1016/s0896-6273(03)00639-1
4
BeurgM.MichalskiN.SafieddineS.BouleauY.SchneggenburgerR.ChapmanE. R.et al. (2010). Control of exocytosis by synaptotagmins and otoferlin in auditory hair cells. J. Neurosci.30, 13281–13290. 10.1523/jneurosci.2528-10.2010
5
BeutnerD.VoetsT.NeherE.MoserT. (2001). Calcium dependence of exocytosis and endocytosis at the cochlear inner hair cell afferent synapse. Neuron29, 681–690. 10.1016/s0896-6273(01)00243-4
6
BorstJ. G.SakmannB. (1996). Calcium influx and transmitter release in a fast CNS synapse. Nature383, 431–434. 10.1038/383431a0
7
BrandtA.KhimichD.MoserT. (2005). Few CaV1.3 channels regulate the exocytosis of a synaptic vesicle at the hair cell ribbon synapse. J. Neurosci.25, 11577–11585. 10.1523/jneurosci.3411-05.2005
8
CarabelliV.Hernández-GuijoJ. M.BaldelliP.CarboneE. (2001). Direct autocrine inhibition and cAMP-dependent potentiation of single L-type Ca2+ channels in bovine chromaffin cells. J. Physiol.532, 73–90. 10.1111/j.1469-7793.2001.0073g.x
9
CarrC. E.MacleodK. M. (2010). Microseconds matter. PLoS Biol.8:e1000405. 10.1371/journal.pbio.1000405
10
CeñaV.StutzinA.RojasE. (1989). Effects of calcium and Bay K-8644 on calcium currents in adrenal medullary chromaffin cells. J. Membr. Biol.112, 255–265. 10.1007/bf01870956
11
ChapochnikovN. M.TakagoH.HuangC. H.PangršičT.KhimichD.NeefJ.et al. (2014). Uniquantal release through a dynamic fusion pore is a candidate mechanism of hair cell exocytosis. Neuron83, 1389–1403. 10.1016/j.neuron.2014.08.003
12
ChoS.LiG. L.von GersdorffH. (2011). Recovery from short-term depression and facilitation is ultrafast and Ca2+ dependent at auditory hair cell synapses. J. Neurosci.31, 5682–5692. 10.1523/jneurosci.5453-10.2011
13
DulonD.SafieddineS.JonesS. M.PetitC. (2009). Otoferlin is critical for a highly sensitive and linear calcium-dependent exocytosis at vestibular hair cell ribbon synapses. J. Neurosci.29, 10474–10487. 10.1523/jneurosci.1009-09.2009
14
FedchyshynM. J.WangL. (2005). Developmental transformation of the release modality at the calyx of Held synapse. J. Neurosci.25, 4131–4140. 10.1523/jneurosci.0350-05.2005
15
FuchsP. A. (2005). Time and intensity coding at the hair cell’s ribbon synapse. J. Physiol.566, 7–12. 10.1113/jphysiol.2004.082214
16
GlowatzkiE.FuchsP. A. (2002). Transmitter release at the hair cell ribbon synapse. Nat. Neurosci.5, 147–154. 10.1038/nn796
17
GoutmanJ. D. (2012). Transmitter release from cochlear hair cells is phase locked to cyclic stimuli of different intensities and frequencies. J. Neurosci.32, 17025–17035. 10.1523/jneurosci.0457-12.2012
18
GoutmanJ. D.GlowatzkiE. (2007). Time course and calcium dependence of transmitter release at a single ribbon synapse. Proc. Natl. Acad. Sci. U S A104, 16341–16346. 10.1073/pnas.0705756104
19
GrantL.YiE.GlowatzkiE. (2010). Two modes of release shape the postsynaptic response at the inner hair cell ribbon synapse. J. Neurosci.30, 4210–4220. 10.1523/jneurosci.4439-09.2010
20
GraydonC. W.ChoS.DiamondJ. S.KacharB.von GersdorffH.GrimesW. N. (2014). Specialized postsynaptic morphology enhances neurotransmitter dilution and high-frequency signaling at an auditory synapse. J. Neurosci.34, 8358–8372. 10.1523/jneurosci.4493-13.2014
21
GraydonC. W.ChoS.LiG. L.KacharB.von GersdorffH. (2011). Sharp Ca2+ nanodomains beneath the ribbon promote highly synchronous multivesicular release at hair cell synapses. J. Neurosci.31, 16637–16650. 10.1523/JNEUROSCI.1866-11.2011
22
HeilP.NeubauerH. (2010). Summing across different active zones can explain the quasi-linear Ca-dependencies of exocytosis by receptor cells. Front. Synaptic Neurosci.2:148. 10.3389/fnsyn.2010.00148
23
HessP.LansmanJ. B.TsienR. W. (1984). Different modes of Ca2+ channel gating behaviour favoured by dihydropyridine Ca2+ agonists and antagonists. Nature311, 538–544. 10.1038/311538a0
24
JarskyT.TianM.SingerJ. H. (2010). Nanodomain control of exocytosis is responsible for the signaling capability of a retinal ribbon synapse. J. Neurosci.30, 11885–11895. 10.1523/jneurosci.1415-10.2010
25
JohnsonS. L.BeurgM.MarcottiW.FettiplaceR. (2011). Prestin-driven cochlear amplification is not limited by the outer hair cell membrane time constant. Neuron70, 1143–1154. 10.1016/j.neuron.2011.04.024
26
JohnsonS. L.FranzC.KnipperM.MarcottiW. (2009). Functional maturation of the exocytotic machinery at gerbil hair cell ribbon synapses. J. Physiol.587, 1715–1726. 10.1113/jphysiol.2009.168542
27
JohnsonS. L.FranzC.KuhnS.FurnessD. N.RüttigerL.MünknerS.et al. (2010). Synaptotagmin IV determines the linear Ca2+ dependence of vesicle fusion at auditory ribbon synapses. Nat. Neurosci.13, 45–52. 10.1038/nn.2456
28
JohnsonS. L.KennedyH. J.HolleyM. C.FettiplaceR.MarcottiW. (2012). The resting transducer current drives spontaneous activity in prehearing mammalian cochlear inner hair cells. J. Neurosci.32, 10479–10483. 10.1523/jneurosci.0803-12.2012
29
JohnsonS. L.MarcottiW. (2008). Biophysical properties of CaV1.3 calcium channels in gerbil inner hair cells. J. Physiol.586, 1029–1042. 10.1113/jphysiol.2007.145219
30
JohnsonS. L.MarcottiW.KrosC. J. (2005). Increase in efficiency and reduction in Ca2+ dependence of exocytosis during development of mouse inner hair cells. J. Physiol.563, 177–191. 10.1113/jphysiol.2004.074740
31
KampT. J.HellJ. W. (2000). Regulation of cardiac L-type calcium channels by protein kinase A and protein kinase C. Circ. Res.87, 1095–1102. 10.1161/01.res.87.12.1095
32
KeenE. C.HudspethA. J. (2006). Transfer characteristics of the hair cell’s afferent synapse. Proc. Natl. Acad. Sci. U S A103, 5537–5542. 10.1073/pnas.0601103103
33
KhimichD.NouvianR.PujolR.Tom DieckS.EgnerA.GundelfingerE. D.et al. (2005). Hair cell synaptic ribbons are essential for synchronous auditory signalling. Nature434, 889–894. 10.1038/nature03418
34
KimM. H.LiG. L.von GersdorffH. (2013). Single Ca2+ channels and exocytosis at sensory synapses. J. Physiol.591, 3167–3178. 10.1113/jphysiol.2012.249482
35
KöpplC. (1997). Phase locking to high frequencies in the auditory nerve and cochlear nucleus magnocellularis of the barn owl, Tyto alba. J. Neurosci.17, 3312–3321.
36
LiG. L.ChoS.von GersdorffH. (2014). Phase-locking precision is enhanced by multiquantal release at an auditory hair cell ribbon synapse. Neuron83, 1404–1417. 10.1016/j.neuron.2014.08.027
37
LiG. L.KeenE.Andor-ArdòD.HudspethA. J.von GersdorffH. (2009). The unitary event underlying multiquantal EPSCs at a hair cell’s ribbon synapse. J. Neurosci.29, 7558–7568. 10.1523/JNEUROSCI.0514-09.2009
38
LibermanM. C. (1978). Auditory-nerve response from cats raised in a low-noise chamber. J. Acoust. Soc. Am.63, 442–455. 10.1121/1.381736
39
MatthewsG.SterlingP. (2008). Evidence that vesicles undergo compound fusion on the synaptic ribbon. J. Neurosci.28, 5403–5411. 10.1523/jneurosci.0935-08.2008
40
McAlpineD. (2005). Creating a sense of auditory space. J. Physiol.566, 21–28. 10.1113/jphysiol.2005.083113
41
MeyerA. C.FrankT.KhimichD.HochG.RiedelD.ChapochnikovN. M.et al. (2009). Tuning of synapse number, structure and function in the cochlea. Nat. Neurosci.12, 444–453. 10.1038/nn.2293
42
MoezziB.IannellaN.McDonnellM. D. (2014). Modeling the influence of short term depression in vesicle release and stochastic calcium channel gating on auditory nerve spontaneous firing statistics. Front. Comput. Neurosci.8:163. 10.3389/fncom.2014.00163
43
MooreD. R. (1991). Anatomy and physiology of binaural hearing. Audiology30, 125–134. 10.3109/00206099109072878
44
MoserT.BeutnerD. (2000). Kinetics of exocytosis and endocytosis at the cochlear inner hair cell afferent synapse of the mouse. Proc. Natl. Acad. Sci. U S A97, 883–888. 10.1073/pnas.97.2.883
45
MoserT.NeefA.KhimichD. (2006). Mechanisms underlying the temporal precision of sound coding at the inner hair cell ribbon synapse. J. Physiol.576, 55–62. 10.1113/jphysiol.2006.114835
46
MurphyG. J.GlickfeldL. L.BalsenZ.IsaacsonJ. S. (2004). Sensory neuron signaling to the brain: properties of transmitter release from olfactory nerve terminals. J. Neurosci.24, 3023–3030. 10.1523/jneurosci.5745-03.2004
47
NeherE. (1998). Vesicle pools and Ca2+ microdomains: new tools for understanding their roles in neurotransmitter release. Neuron20, 389–399. 10.1016/s0896-6273(00)80983-6
48
NowyckyM. C.FoxA. P.TsienR. W. (1985). Long-opening mode of gating of neuronal calcium channels and its promotion by the dihydropyridine calcium agonist Bay K 8644. Proc. Natl. Acad. Sci. U S A82, 2178–2182. 10.1073/pnas.82.7.2178
49
OheimM.KirchhoffF.StühmerW. (2006). Calcium microdomains in regulated exocytosis. Cell Calcium40, 423–439. 10.1016/j.ceca.2006.08.007
50
PalmerA. R.RussellI. J. (1986). Phase-locking in the cochlear nerve of the guinea-pig and its relation to the receptor potential of inner hair-cells. Hear. Res.24, 1–15. 10.1016/0378-5955(86)90002-x
51
PangrsicT.LasarowL.ReuterK.TakagoH.SchwanderM.RiedelD.et al. (2010). Hearing requires otoferlin-dependent efficient replenishment of synaptic vesicles in hair cells. Nat. Neurosci.13, 869–876. 10.1038/nn.2578
52
PicklesJ. O. (1996). An Introduction to the Physiology of Hearing.San Diego: Academic Press Inc.
53
PlatzerJ.EngelJ.Schrott-FischerA.StephanK.BovaS.ChenH.et al. (2000). Congenital deafness and sinoatrial node dysfunction in mice lacking class D L-type Ca2+ channels. Cell102, 89–97. 10.1016/s0092-8674(00)00013-1
54
RoseJ. E.BruggeJ. F.AndersonD. J.HindJ. E. (1967). Phase-locked response to low-frequency tones in single auditory nerve fibers of the squirrel monkey. J. Neurophysiol.30, 769–793.
55
RossingT. D. (2007). Springer Handbook of Acoustics.New York: Springer.
56
RouxI.SafieddineS.NouvianR.GratiM.SimmlerM. C.BahloulA.et al. (2006). Otoferlin, defective in a human deafness form, is essential for exocytosis at the auditory ribbon synapse. Cell127, 277–289. 10.1016/j.cell.2006.08.040
57
RussellI. J.SellickP. M. (1978). Intracellular studies of hair cells in the mammalian cochlea. J. Physiol.284, 261–290. 10.1113/jphysiol.1978.sp012540
58
RutherfordM. A.ChapochnikovN. M.MoserT. (2012). Spike encoding of neurotransmitter release timing by spiral ganglion neurons of the cochlea. J. Neurosci.32, 4773–4789. 10.1523/jneurosci.4511-11.2012
59
SafieddineS.WentholdR. J. (1999). SNARE complex at the ribbon synapses of cochlear hair cells: analysis of synaptic vesicle- and synaptic membrane-associated proteins. Eur. J. Neurosci.11, 803–812. 10.1046/j.1460-9568.1999.00487.x
60
SchneeM. E.Castellano-MuñozM.RicciA. J. (2013). Response properties from turtle auditory hair cell afferent fibers suggest spike generation is driven by synchronized release both between and within synapses. J. Neurophysiol.110, 204–220. 10.1152/jn.00121.2013
61
SingerJ. H.LassovàL.VardiN.DiamondJ. S. (2004). Coordinated multivesicular release at a mammalian ribbon synapse. Nat. Neurosci.7, 826–833. 10.1038/nn1280
62
StanleyE. F. (1993). Single calcium channels and acetylcholine release at a presynaptic nerve terminal. Neuron11, 1007–1011. 10.1016/0896-6273(93)90214-c
63
SuryanarayananA.SlaughterM. M. (2006). Synaptic transmission mediated by internal calcium stores in rod photoreceptors. J. Neurosci.26, 1759–1766. 10.1523/jneurosci.3895-05.2006
64
TabernerA. M.LibermanM. C. (2005). Response properties of single auditory nerve fibers in the mouse. J. Neurophysiol.93, 557–569. 10.1152/jn.00574.2004
65
ThoresonW. B.RablK.Townes-AndersonE.HeidelbergerR. (2004). A highly Ca2+-sensitive pool of vesicles contributes to linearity at the rod photoreceptor ribbon synapse. Neuron42, 595–605. 10.1016/s0896-6273(04)00254-5
66
TrussellL. O. (2002). Transmission at the hair cell synapse. Nat. Neurosci.5, 85–86. 10.1038/nn0202-85
67
VincentP. F.BouleauY.SafieddineS.PetitC.DulonD. (2014). Exocytotic machineries of vestibular type I and cochlear ribbon synapses display similar intrinsic otoferlin-dependent Ca2+ sensitivity but a different coupling to Ca2+ channels. J. Neurosci.34, 10853–10869. 10.1523/jneurosci.0947-14.2014
68
von GersdorffH. (2001). Synaptic ribbons: versatile signal transducers. Neuron29, 7–10. 10.1016/s0896-6273(01)00175-1
69
WeberA. M.WongF. K.TuffordA. R.SchlichterL. C.MatveevV.StanleyE. F. (2010). N-type Ca2+ channels carry the largest current: implications for nanodomains and transmitter release. Nat. Neurosci.13, 1348–1350. 10.1038/nn.2657
70
WolfM.EberhartA.GlossmannH.StriessnigJ.GrigorieffN. (2003). Visualization of the domain structure of an L-type Ca2+ channel using electron cryo-microscopy. J. Mol. Biol.332, 171–182. 10.1016/s0022-2836(03)00899-4
71
WongA. B.RutherfordM. A.GabrielaitisM.PangrsicT.GöttfertF.FrankT.et al. (2014). Developmental refinement of hair cell synapses tightens the coupling of Ca2+ influx to exocytosis. EMBO J.33, 247–264. 10.1002/embj.201387110
72
ZampiniV.JohnsonS. L.FranzC.KnipperM.HolleyM. C.MagistrettiJ.et al. (2013). Burst activity and ultrafast activation kinetics of CaV1.3 Ca2+ channels support presynaptic activity in adult gerbil hair cell ribbon synapses. J. Physiol.591, 3811–3820. 10.1113/jphysiol.2013.251272
73
ZampiniV.JohnsonS. L.FranzC.KnipperM.HolleyM. C.MagistrettiJ.et al. (2014). Fine tuning of CaV1.3 Ca2+ channel properties in adult inner hair cells positioned in the most sensitive region of the Gerbil cochlea. PLoS One9:e113750. 10.1371/journal.pone.0113750
74
ZampiniV.JohnsonS. L.FranzC.LawrenceN. D.MünknerS.EngelJ.et al. (2010). Elementary properties of CaV1.3 Ca(2+) channels expressed in mouse cochlear inner hair cells. J. Physiol.588, 187–199. 10.1113/jphysiol.2009.181917
75
ZampiniV.RüttigerL.JohnsonS. L.FranzC.FurnessD. N.WaldhausJ.et al. (2011). Eps8 regulates hair bundle length and functional maturation of mammalian auditory hair cells. PLoS Biol.9:e1001048. 10.1371/journal.pbio.1001048
Summary
Keywords
inner hair cell, Ca2+ channel, patch-clamp, phase locking, cochlea, ribbon synapse, multivesicular release, Eps8
Citation
Magistretti J, Spaiardi P, Johnson SL and Masetto S (2015) Elementary properties of Ca2+ channels and their influence on multivesicular release and phase-locking at auditory hair cell ribbon synapses. Front. Cell. Neurosci. 9:123. doi: 10.3389/fncel.2015.00123
Received
10 February 2015
Accepted
17 March 2015
Published
08 April 2015
Volume
9 - 2015
Edited by
Gerald W. Zamponi, University of Calgary, Canada
Reviewed by
Lu-Yang Wang, University of Toronto, Canada; Martin Heine, Leibniz Institute for Neurobiology, Germany
Copyright
© 2015 Magistretti, Spaiardi, Johnson and Masetto.
This is an open-access article distributed under the terms of the Creative Commons Attribution License (CC BY). The use, distribution and reproduction in other forums is permitted, provided the original author(s) or licensor are credited and that the original publication in this journal is cited, in accordance with accepted academic practice. No use, distribution or reproduction is permitted which does not comply with these terms.
*Correspondence: Sergio Masetto, Department of Brain and Behavioral Sciences, University of Pavia, Via Forlanini 6, Pavia 27100, Italy smasetto@unipv.it
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