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The Journal of Neuroscience, May 15, 1998, 18(10):3715-3724

Calcium Currents and Calcium Signaling in Rod Bipolar Cells of Rat Retinal Slices

Dario A. Protti and Isabel Llano

Arbeitsgruppe Zelluläre Neurobiologie, Max-Planck-Institut für biophysikalische Chemie, 37070 Göttingen, Germany

	ABSTRACT

Top Abstract Introduction Materials & Methods Results Discussion References

Combined electrophysiological and imaging techniques were used to study calcium currents (I_Ca) and their sites of origin at rod bipolar cells in rat retinal slices. We report here for the first time the successful whole-cell patch-clamp recording from presynaptic boutons that were compared with somatic recordings. TTX-resistant inward currents were elicited in response to depolarization. The kinetic and pharmacological properties of I_Ca were very similar for recordings obtained from the soma and the presynaptic terminals. I_Ca activated maximally between 30 and 20 mV was enhanced by Bay K 8644 and was blocked by isradipine and nifedipine. Peak amplitude and time to peak were 31.3 ± 1.2 pA and 3.2 ± 0.2 msec with somatic recordings (n = 54), whereas the corresponding values were 31.6 ± 6.1 pA and 3.2 ± 0.7 msec in recordings obtained directly from terminals (n = 6). I_Ca showed little inactivation during sustained depolarizations. No T-type I_Ca was observed with depolarizations from 90 mV. Concomitant with Ca²⁺ entry, depolarization induced the appearance of transient outward currents that resembled IPSCs and were blocked by GABA and glycine receptor antagonists, suggesting that they arise from activation of amacrine feedback synapses. Upon depolarization, intracellular Ca²⁺ ([Ca²⁺]_i) rises were restricted to the presynaptic terminals with no somatic or axonal changes and were linearly dependent on pulse duration when using a low-affinity Ca²⁺ indicator. In cone bipolar cells, I_Ca inactivated markedly, and [Ca²⁺]_i rises occurred in the axon, as well as in the presynaptic terminals.

Key words: retina; bipolar cells; calcium channels; presynaptic terminal; calcium imaging; CNS slices; reciprocal synapses

	INTRODUCTION

Top Abstract Introduction Materials & Methods Results Discussion References

Retinal bipolar cells are glutamatergic interneurons that transmit light-induced photoreceptor signals to amacrine and ganglion cells in the inner plexiform layer (IPL) via chemical synapses. On the basis of morphological and physiological criteria, two different types of bipolar cells can be distinguished: the cone bipolar cells (CBCs), which are subdivided into several classes, and the rod bipolar cells (RBCs). Unlike most mammalian neurons, bipolar cells do not produce Na⁺-based action potentials. Transmission of signals impinging on their dendrites is reliant on the passive electrotonic spread of the signal to the axonal terminals from which neurotransmitter is released in a graded manner.

To serve diverse physiological functions, channels and receptors are differentially distributed in distinct compartments of these cells. Receptors to neurotransmitters are clustered in dendritic postsynaptic densities in which they bind transmitter released by presynaptic neurons, as is the case for mGluR6 in RBCs (Nomura et al., 1994). In addition, neurotransmitter receptors are also present at different densities in the soma and axon (for an example of NMDA receptor distribution, see Wenzel et al., 1997). They are also found at presynaptic terminals in which bipolar cells receive reciprocal synapses from amacrine cells that exert feedback inhibition on transmitter release (Raviola and Dacheux, 1987; Tachibana and Kaneko, 1987; Zhang et al., 1997).

Because of their pivotal role in transmitter release, Ca²⁺ channels are expected to be present in the synaptic boutons to enable the Ca²⁺ influx required for exocytosis. Indeed, a preferential localization of L-type Ca²⁺ channels has been described in Mb1 bipolar cells of the goldfish retina, which receive a mixed input from cone and rod photoreceptors (Heidelberger and Matthews, 1992; Tachibana et al., 1993; Mennerick et al., 1997). Moreover, in dissociated rat bipolar cells L-type channels mediate K⁺-evoked intracellular Ca²⁺ ([Ca²⁺]_i) rises in presynaptic terminals (Pan and Lipton, 1995). Work in isolated mouse retinal bipolar cells has suggested that calcium currents (I_Ca) are carried by low-voltage-activated T-type channels (Kaneko et al., 1989). It has recently been reported, however, that in addition to the T-type I_Ca, a dihydropyridines (DHP)-sensitive component of I_Ca is present in bipolar cells from mouse retinal slices (de la Villa et al., 1998).

The characterization of the functional Ca²⁺ channel types present in the diverse neuronal elements in intact slices is a crucial requirement for the elucidation of the synaptic processing pathways in the retina. Our experiments were performed to identify Ca²⁺ channel type and spatial distribution in RBCs in rat retinal slices. Through the combined use of whole-cell voltage-clamp and fluorometric Ca²⁺ imaging and direct recordings from synaptic terminals, we have found that Ca²⁺ influx occurs via L-type channels and that the ensuing [Ca²⁺]_i rises are restricted to presynaptic terminals.

A preliminary report of this work has been presented in abstract form (Protti and Llano, 1997).

	MATERIALS AND METHODS

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Retinal vertical slices were prepared from 4- to 7-week-old rats, following procedures previously described by Protti et al. (1997). The standard external solution, bicarbonate-buffered saline (BBS), consisted of (in mM): 125 NaCl, 2.5 KCl, 2 CaCl₂, 1 MgCl₂, 1.25 NaH₂PO₄, 26 NaHCO₃, and 10 glucose, pH 7.4 when equilibrated with a mixture of 95% O₂ and 5% CO₂. Most of the experiments were performed with a Cs gluconate (CsGlu)-based solution containing (in mM): 132 CsGlu, 5 CsCl, 20 Cs-HEPES, 4.6 MgCl₂, 0.1 EGTA, 0.4 Na-GTP, and 4 Na-ATP, pH 7.3. In some cases, K⁺ replaced Cs⁺ as the main cation, and Cl was the main anion. In some experiments, recording pipettes contained either Lucifer yellow (0.5 mg/ml) or neurobiotin (2 mg/ml; Vector Laboratories, Burlingame, CA). All other chemicals were purchased from Sigma (St. Louis, MO).

Electrophysiological recordings. Experiments were performed with the tight-seal whole-cell recording (wcr) configuration of the patch-clamp technique (Hamill et al., 1981). All experiments were done at room temperature (20-25°C) using an upright microscope (Zeiss Axioskop) equipped with Nomarski differential interference contrast optics and a water immersion objective (63×, 0.9 numerical aperture). Recordings were obtained from the somata, as well as from axonal terminals of bipolar cells located in the outer part of the inner nuclear layer (INL), using an EPC-9 amplifier (Heka Electronics). Borosilicate glass pipettes with resistance of 5-8 M were used for somatic recordings, whereas those used for terminal recordings had values of 18-20 M. Series resistances ranged from 14 to 20 M in somatic recordings and from 38 to 60 M in terminal recordings. Leak and capacitive currents were subtracted using the average of six hyperpolarizing pulses, and series resistance was compensated (nominally 70-80%). Membrane potential values were corrected for junction potential. The chamber was perfused at 1-1.5 ml/min with BBS. To improve the signal-to-noise ratio, traces were averaged for each experimental condition. For electrophysiological studies, as well as during [Ca²⁺]_i imaging experiments, recordings were discontinued if the holding current at 70 mV exceeded 30 pA.

After electrophysiological recordings, histological examination of neurobiotin-filled cells was performed as described by Protti et al. (1997).

Fluorometric calcium imaging. Changes in [Ca²⁺]_i were detected as changes in the fluorescence intensity of one of the following Ca²⁺-sensitive probes included in the patch pipette: 200 µM Oregon green 488 BAPTA-5N (OG5) or 50 µM Oregon green 488 BAPTA-1 (OG1). No EGTA was present in the CsGlu solution. Digital fluorescence images were obtained with image acquisition systems and a monochromatic light source for fluorescence excitation (T.I.L.L. Photonics, Planegg, Germany). The excitation pathway consisted of a 75 W Xe lamp focused on a scanning monochromator and coupled to the microscope by a quartz fiber and a lens. The dichroic mirror and high-pass emission filter had center wavelengths at 505 and 507 nm, respectively. Two types of peltier-cooled, slow-scan CCD cameras were used in the present work: (1) a camera based on a Thompson 7863 frame transfer chip with 384 × 286 pixels (pixel size was 0.36 µm after 63× magnification), and (2) a PCO SensiCam camera with 640 × 480 pixels (pixel size was 0.25 µm after 63× magnification). Both cameras were connected to 12 bit analog-to-digital converters and had sufficient dynamic range to ensure that no saturation occurred when imaging the cell structures with large fluorescence signals, such as the cell soma. In the present study, pixel binning (4 × 4) was performed with type 1 to achieve a fast acquisition rate and to improve the signal-to-noise ratio when low concentrations of the high-affinity dye OG1 were used. Type 2 was used to acquire full images (no binning performed) and to study the spatial distribution of signals with higher spatial resolution.

The standard protocol to study [Ca²⁺]_i transients consisted of acquiring a sequence of 20 images at regular intervals. Four images were taken while the cell was held at 70 mV, and a single depolarizing voltage step was applied at the end of the fourth image. Images were integrated from 10 to 70 msec (see Results and figure legends). Fluorescence changes were analyzed off-line by measuring the average fluorescence in small regions of interest (ROIs; ~1-2 µm²) and converting it to the percent of change in fluorescence: F/F_o = 100 × (F  F_r)/(F_r  B), in which F is the measured fluorescence signal at any given time, F_r is the average fluorescence from four consecutive images preceding the voltage step, and B is the average value of the background fluorescence from four regions located in the periphery of the visual field and of equal size to the cellular ROIs. As discussed by Llano et al. (1997), the F/F_o ratio faithfully reflects changes in [Ca²⁺]_i. Background values were stable during each experimental run, and the basal counts in the various ROIs analyzed were unambiguously distinguishable from the background. The mean ± SEM for the ratio of prestimuli counts/background counts was 1.56 ± 0.1 for OG5 (n = 20) and 3.2 ± 0.5 for OG1 (n = 10).

Images displayed in the figures correspond to raw prestimuli and poststimuli data (i.e., no subtraction of background counts, averaging, or masking has been performed). They are displayed with a pseudocolor scale such that the smallest fluorescent signals are clearly apparent, whereas signals in the soma are saturated. But we stress again that the original data in which the calculation of F/F_o is based are not saturated.

To verify cell identity, long-exposure (500 msec) images of cells filled with fluorescent Ca²⁺ indicators or Lucifer yellow were acquired at different focal planes at the end of the experiments. Photomontages were constructed using Adobe Photoshop software (see Figs. 1, 4, 8). Such strong illumination can lead to cell damage, as denoted by the development of large holding currents and axonal swellings.

	RESULTS

Top Abstract Introduction Materials & Methods Results Discussion References

Identification of RBCs

RBCs were identified from their position in the outermost part of the INL using Nomarski optics. Occasionally, their axon could be sighted as a single process running along the IPL. Further corroboration of cell type was established by filling cells with Lucifer yellow or staining with neurobiotin. Figure 1A shows a transmitted light picture of a 180-µm-thick slice with a patch pipette on an RBC. The same cell can be observed in Figure 1B, 10 min after establishing the wcr when dialysis has taken place. Its axon descends straight along the IPL and branches into three small processes in strata 5 of sublamina b of the IPL close to the ganglion cell layer, a pattern typical of rat RBCs (Euler and Wässle, 1995). Under wcr, current relaxations elicited by 10 mV hyperpolarizing pulses deviated from monoexponential or biexponential functions, suggesting a multicompartment equivalent electrical circuit. Nonetheless, a large fraction of the current relaxation, presumably corresponding to the somatodendritic compartment, could be compensated by the slow capacitance circuit of the amplifier, yielding values of 3.29 ± 0.09 pF (n = 51).

View larger version (44K): [in this window] [in a new window]   Figure 1.   Identification of RBCs in rat retinal slices. A, Transmitted light image of a retinal slice preparation with the recording pipette placed on a cell body located in the inner nuclear layer. Arrows indicate the approximate boundaries of the different layers observed. INL, Inner nuclear layer; IPL, inner plexiform layer; GCL, ganglion cell layer. B, The same cell with its axon descending straight along the IPL and branching into three small processes in the outer part of the IPL (close to the ganglion cell layer) can be observed 10 min after breaking into the cell. A photomontage of images obtained at three different focal planes is shown. The cell was filled with 200 µM OG5. Scale bar applies to A and B.

Calcium currents in RBCs

In agreement with previous observations (Kaneko et al., 1989; Karschin and Wässle, 1990; Klumpp et al., 1995), we found that in cells dialyzed with KCl-based internal solutions, robust slowly inactivating outward currents were activated by depolarizations to values greater than 20 mV applied from a holding potential of 70 mV. No net inward currents were observed in these ionic conditions (data not shown).

To study I_Ca, patch pipettes were filled with CsGlu to eliminate K⁺ efflux and to avoid possible contamination of the inward current by Ca²⁺-dependent Cl currents. These Cl currents were observed in preliminary experiments and have been previously described in goldfish bipolar cells (Okada et al., 1995). Figure 2A shows typical voltage-gated currents recorded with CsGlu pipettes. The currents are inward for potentials between 50 and 0 mV and outward at positive potentials. Their activation threshold was between 50 and 40 mV, and peak amplitudes were reached between 30 and 20 mV in the presence of 2 mM external Ca²⁺ (Fig. 2B, filled circles). The peak amplitude and time to peak were 31.3 ± 1.2 pA and 3.2 ± 0.2 msec, respectively (n = 54). As shown in Figure 2B, even in cells dialyzed with CsGlu, a significant outward current developed for depolarizations >10 mV. Such currents are likely attributable to Cs⁺ flowing through K⁺ channels because they are strongly reduced when the cells are bathed in Ba²⁺, a well known blocker of several K⁺ channels (see the I-V relationship in Fig. 2B, triangles). The inward currents were resistant to the sodium channel blocker TTX (400 nM) and were abolished on removal of external Ca²⁺, and their magnitude was increased when 5 mM Ba²⁺ was used as charge carrier (Fig. 2C).

View larger version (33K): [in this window] [in a new window]   Figure 2.   ICa in rod bipolar cells. A, Currents recorded under somatic whole-cell voltage clamp in a RBC dialyzed with CsGlu. Depolarizing pulses were applied from a holding potential of 70 mV in 20 mV increments. B, Pooled data on the current-voltage relationship obtained in RBCs dialyzed with CsGlu in 2 mM external Ca2+ (filled circles; n = 8) and in 5 mM external Ba2+ (open triangles; n = 5). Error bars indicate SEM. In both groups the activation threshold for the inward current was at 40 mV, and peak amplitudes were reached at 20 mV. Note the decrease in outward current when cells were bathed in external Ba2+. C, Comparison of the inward currents elicited by pulses to 30 mV (Vh, 70 mV) in an RBC when the slice is perfused with 2 mM Ca2+ or 5 mM Ba2+. Each trace is the average of 24 individual records. D, Negligible inactivation of ICa in RBCs. Currents were elicited by depolarizing pulses to 20 mV (Vh, 70 mV) of 50, 250, and 500 msec duration. Each trace is the average of 24 records.

To explore the inactivation properties of I_Ca, pulses of varying duration (to 20 mV) were applied. As shown in Figure 2D, I_Ca decay is small, even for 500 msec pulses. For 100 msec pulses, I_Ca decayed to 91.3 ± 2.2% of its peak value (n = 7). Because the intracellular solution contained no exogenous Ca²⁺ buffer, these results indicate that Ca²⁺-dependent inactivation of I_Ca is minor in RBCs. After replacing external Ca²⁺ with Ba²⁺, the inactivation rate of the Ba²⁺ current was slightly smaller, with the inward current declining to 96.2 ± 0.86% of its peak after a 100 msec depolarizing pulse (n = 6). A remarkable feature of I_Ca was its stability: some cells were recorded for 1 hr without any noticeable decline in peak current amplitude.

The properties described above are typical of high-voltage-activated (HVA) Ca²⁺ currents. Depolarizing steps from 90 mV failed to elicit a transient current component, indicating the lack of low-voltage-activated T-type currents (data not shown).

Pharmacology of calcium currents

The biophysical properties of different HVA currents, as well as the use of specific neurotoxins and blockers, has led to the identification of several Ca²⁺ channel types, namely L, N, P/Q, and R types (Zhang et al., 1993; McCleskey, 1994; Randall and Tsien, 1995; Uchitel, 1997). L-type Ca²⁺ channels inactivate slowly and are sensitive to both a family of organic compounds (the DHPs that include agonists and antagonist) and to the neuropeptide calciseptine. N-type Ca²⁺ channels have an intermediate inactivation rate and are blocked by the neurotoxin -conotoxin GVIA. P/Q-type Ca²⁺ channels inactivate very slowly. They are insensitive to DHPs and to -conotoxin GVIA, but are sensitive to the neuropeptide -agatoxin IVA at different doses for each channel type. R-type Ca²⁺ channels are resistant to all of the blockers mentioned above.

Consistent with the aforementioned slow inactivation rate that characterizes L-type I_Ca, we found that the currents through Ca²⁺ channels in RBCs were effectively blocked by isradipine or nifedipine (1-10 µM) in all cells tested. The DHP antagonists blocked I_Ca by 92 ± 1.5% (n = 8). As shown in Figure 3A, the small residual current recorded in the presence of DHP antagonists had the same time course as the control current. The block was only partially reversible, probably attributable to the length of time required to wash out drugs from slices. As expected for L-type Ca²⁺ channels, currents were enhanced by the DHP agonist Bay K 8644 (Fig. 3B). In the presence of Bay K 8644, tail currents had slower kinetics. This could reflect a genuine kinetic change, which is known to occur in the presence of this drug (Nowycky et al., 1985), as well as space-clamp failure on repolarization attributable to the increased current density. Thus, the large degree of block by DHP antagonists, the sensitivity to Bay K 8644, and the kinetics of the currents recorded in the presence of DHP antagonists indicate that L-type Ca²⁺ channels mediate the totality of I_Ca in RBCs. Hence, the effects of other non-L-type Ca²⁺ channel antagonists were not explored.

View larger version (22K): [in this window] [in a new window]   Figure 3.   Pharmacological profile of the inward currents. A, The dihydropyridine antagonist isradipine (10 µM) blocks the ICa elicited by a depolarizing step to 30 mV (Vh, 70 mV). Each trace is the average of 24 records. B, ICa was increased after bath application of Bay K 8644 (10 µM), a specific agonist of L-type Ca2+ channels. Note the increase in amplitude and slower decay of the tail upon return to the holding potential of 70 mV. Each trace is the average of 36 records. C, Evidence for the activation of reciprocal synapses. Current fluctuations superimposed upon depolarization-evoked ICa in control external saline (top trace) and after bath perfusion with antagonists of GABA and glycine receptors (bottom trace). Each current record is the result of a single depolarizing pulse to 0 mV. Internal solution for A-C was CsGlu.

Depolarizing pulses to RBCs sometimes elicited transient current fluctuations superimposed on the pulse-evoked inward current. Such fluctuations appeared as outward deflections in the current trace. The probability of obtaining these events was higher shortly after pulse onset, but they could be observed throughout the depolarization (Fig. 3C). The temporal profile of these events resembled that of inhibitory synaptic currents recorded under low internal Cl, suggesting that they could originate from the concomitant activity of reciprocal synapses formed between RBCs and amacrine cells. In accord with this hypothesis, these current fluctuations were sensitive to an antagonist cocktail of bicuculline, 3-APMPA, and strychnine (GABA_A, GABA_C, and glycine antagonists, respectively), as shown by the example in Figure 3C (n = 3).

Terminal recordings

In goldfish Mb1 bipolar cells with giant synaptic terminals, most of I_Ca is carried through L-type Ca²⁺ channels at the presynaptic terminal (Heidelberger and Matthews, 1992; Tachibana et al., 1993). Because of the small size of synaptic boutons, direct recordings from presynaptic terminals in mammalian CNS slice preparations have been limited to the calyces of Held (Barnes-Davies and Forsythe, 1995; Borst et al., 1995; Helmchen et al., 1997) and more recently to terminals of cerebellar basket cells (Southan and Robertson, 1998). Rat RBCs possess relatively large presynaptic boutons (2.5-4 µm) that could allow direct recordings providing more accurate voltage control and the possibility of a straight assay for exocytosis through membrane capacitance measurements. We set out to test the feasibility of direct terminal recordings from RBCs by using a similar approach to that used for dendritic recordings in several neuronal cells, i.e., Nomarski optics to improve terminal visualization and small-tip diameter patch pipettes to avoid damage to the small structure. The price to pay for small pipette tips is a high-access resistance that might compromise voltage clamp. Nevertheless, the small maximum amplitude of I_Ca as observed in standard (somatic) recordings predicts an error of 3 mV for recordings with access resistance of 60 M. Furthermore, because L-type I_Ca activates slowly, the temporal course of these currents may not be distorted by the filtering imposed by the high-access resistance.

Occasionally, when the retinal tissue was fully embedded in agar, i.e., it had no vitreous attached, slices of sufficient viability could be obtained to allow recording from the boutons of RBCs. It must be remarked, however, that preparations were scarce in which putative terminals could be visualized and high-resistance seals could be formed, and recording from these small structures was a difficult procedure.

Figure 4A illustrates an RBC filled with Lucifer yellow via a patch pipette in the presynaptic terminal. This cell had a large terminal, and both the axon and soma were stained, allowing its positive identification as an RBC. As in the somatic recordings, inward currents were elicited in response to depolarizing pulses ranging from 30 to 10 mV, and outward currents were present at more positive membrane potentials (Fig. 4B). The properties of I_Ca in terminal recordings closely resembled those obtained in somatic recordings: (1) the I-V relationship was typical of HVA Ca²⁺ channels (Fig. 4C); (2) the current had a slow onset (time to peak, 3.2 ± 0.7 msec; n = 6); and (3) the current had little inactivation. The mean value for time to peak, as well as for the peak I_Ca amplitude from terminal recordings (31.6 ± 6.1 pA, n = 6), were indistinguishable from those obtained when recording with a pipette at the soma. As expected for Ca²⁺ channels, no inward currents were observed in Ca²⁺-free medium, and larger currents were obtained with 4 mM external Ba²⁺ (Fig. 4D). Responses to linear ramps (from 70 to 70 mV; 100 mV/sec) overlapped with the I-V relationship (data not shown).

View larger version (67K): [in this window] [in a new window]   Figure 4.   Terminal recordings of ICa obtained with a CsGlu-based internal solution. A, Transmitted light view of a retinal slice (left) in which an RBC has been filled with Lucifer yellow via a recording pipette located on the terminal situated in the most external part of the IPL (right). B, Current records obtained from a different cell under voltage clamp with a patch pipette placed onto the RBC terminal. Depolarizing pulses were applied from a Vh of 70 mV in 20 mV steps. C, Current-voltage relationship for the responses elicited in a terminal recording by depolarizing steps (filled circles; each point is the average of two pulses) (Vh, 70 mV). D, In a different terminal recording, the voltage-gated inward currents were abolished in the absence of external Ca2+, and their magnitude was increased when replacing 2 mM Ca2+ with 4 mM Ba2+. As in the somatic recordings, ICa inactivation was slow. E, ICa elicited by depolarizing steps from a Vh of 70 mV to 10 mV in terminal recording (traces are the average of 24 individual currents; same cell as in A-C) was enhanced by Bay K 8644 (1 µM). Internal solution for A-E was CsGlu.

The pharmacological profile of these currents was also examined. As with somatic I_Ca, they were insensitive to TTX (400 nM) but were effectively blocked by the L-type Ca²⁺ channel blockers nifedipine (10 µM) and isradipine (1-10 µM). As before, Bay K 8644 (1 µM) increased peak current amplitude as well as the magnitude of the tail currents (Fig. 4E). In the presence of Bay K 8644, no escape of voltage control in the tail current was observed contrary to somatic recordings, suggesting a better quality of the space clamp under terminal recording conditions.

Ca²⁺ channel localization

The properties of depolarization-evoked [Ca²⁺]_i rises in the somatodendritic compartment of individual neurons have been well documented (for review, see Regehr and Tank, 1994). More recently, [Ca²⁺]_i rises have been studied in axonal varicosities, branch points, synaptic boutons, and preterminal axonal segments (Borst et al., 1995; Regehr and Atluri, 1995; Callewaert et al., 1996; Mackenzie et al., 1996; Llano et al., 1997).

The data described in previous sections provide tantalizing evidence for the selective localization of L-type Ca²⁺ channels in the synaptic terminals of rat RBCs. To test such a suggestion, [Ca²⁺]_i was monitored through fluorescence imaging with Ca²⁺-sensitive probes of different Ca²⁺ affinity. In the first series of experiments, the low-affinity indicator OG5 (K_d, ~20 µM according to Molecular Probes, Eugene, OR) was used to avoid significant interference of the dye with intrinsic [Ca²⁺]_i buffering. RBCs were dialyzed with the CsGlu solution containing OG5 (200 µM), and the dye was allowed to diffuse for 5 min before applying stimulation protocols. Fluorescence images at different focal planes allowing visualization of the soma, axon, and synaptic terminals were acquired before and after depolarizing pulses. Figure 5 shows a representative experiment in which the focal plane was first optimized for the synaptic terminal (Fig. 5Aa,Ab) and subsequently set to image the soma and axon (Fig. 5Ba,Bb). Images taken before (Fig. 5Aa,Ba) and after (Fig. 5Ab,Bb) a 50 msec depolarizing pulse are displayed. Figure 5C plots the temporal evolution of the F/F_o that reflects changes in [Ca²⁺]_i (see Materials and Methods) at the three different locations. It is clear that the depolarization evokes [Ca²⁺]_i rises exclusively at the synaptic bouton. Neither the cell soma nor the axon increased its [Ca²⁺]_i level. This confinement of the [Ca²⁺]_i rises to the presynaptic terminals was observed in 21 RBCs. The spread of the [Ca²⁺]_i signals along the axon was not systematically examined, owing to the axon continuously changing its depth within the slice as it descends along the IPL. No spread of the [Ca²⁺]_i signal was observed for pulses <100 msec in duration at distances as short as 10 µm from the terminals, however. At presynaptic boutons, the average peak F/F_o for 50 msec depolarizing pulses was 85 ± 13.9% (n = 17).

View larger version (86K): [in this window] [in a new window]   Figure 5.   Spatial distribution of pulse-evoked [Ca2+]i rises detected with the low-affinity dye OG5 (200 µM). A, B, Pseudocolor images of Ca2+-dependent fluorescence at rest (Aa, Ba; Vh, 70 mV) and during a 50 msec pulse to 30 mV (Ab, Bb). A and B were taken at different focal planes optimized for the terminal in A and for the axon in B. Camera exposure time was 20 msec, and cycle time for image acquisition was 52 msec. C, Temporal evolution of the relative changes in fluorescence measured in discrete ROI (see Materials and Methods) as indicated in the image: triangle represents axon, inverted triangle represents soma, and circle represents terminal. The depolarization-evoked change in fluorescence is restricted to the bipolar terminal. In this and the following figures the slices were bathed in the standard control saline (2 mM Ca2+). Pipettes were filled with a CsGlu-based solution (no EGTA) as detailed in Materials and Methods.

As in the case of I_Ca, [Ca²⁺]_i transients in synaptic terminals were unaffected by 400 nM TTX but were almost completely eliminated by 10 µM isradipine (n = 3) and enhanced by 10 µM Bay K (n = 1), confirming that Ca²⁺ influx does indeed occur at the presynaptic terminals through L-type Ca²⁺ channels.

Using OG5, we examined the relationship between [Ca²⁺]_i rise and Ca²⁺ influx. Given the very small decay of I_Ca, this relationship could simply be obtained by varying pulse duration. Figure 6Aa illustrates at high magnification a sequence of images of three boutons acquired every 54 msec. A basal image is shown in the first panel of Figure 6Aa, and the subsequent panels correspond to the first three images after a 50 msec depolarizing pulse. The corresponding F/F_o and I_Ca plots are displayed in Figure 6, Ab and Ac, respectively. In this experiment, as in other cells tested, depolarization-induced [Ca²⁺]_i transients peaked within one image for 10-50 msec pulses, limited by the sampling rate (54 msec/image). For 100-500 msec pulses, [Ca²⁺]_i peaked at the image corresponding to the end of the pulse (Fig. 6B). The relationship between pulse duration and peak F/F_o was linear throughout the range explored (Fig. 7D). For 50 msec pulses, OG5 [Ca²⁺]_i transients decayed to 50% of their maximum at 430 ± 50 msec (n = 14).

View larger version (52K): [in this window] [in a new window]   Figure 6.   Modulation of terminal [Ca2+]i rises by pulse duration. Aa, Time sequence of OG5 pseudocolor images from the synaptic terminal region of an RBC. The first panel corresponds to the fourth image in a series taken at rest (cycle time, 52 msec). A 50 msec depolarization to 0 mV, applied immediately after the end of this image (time, 156-206 msec), elicits substantial increases in fluorescence throughout the terminals that begins to decay when the membrane potential returns to Vh. Ab, Ac, Temporal evolution of the percent of fluorescence change and the corresponding ICa for the experiment shown in Aa. Ba, Bb, Temporal evolution of the percent of fluorescence change and the corresponding ICa for a 250 msec depolarization in the same cell. Note that for a given pulse duration, the pulse-evoked changes in fluorescence have similar magnitudes and time courses in the two terminals analyzed. Internal solution was CsGlu (200 µM OG5, no EGTA).

View larger version (25K): [in this window] [in a new window]   Figure 7.   Properties of the [Ca2+]i rises measured with low- and high-affinity Ca2+ indicators. A, The spatial distribution of the relative changes in fluorescence reported by the high-affinity indicator OG1 (50 µM) is similar to that observed with OG5. A 50 msec depolarization to 20 mV from a Vh of 70 mV results in increases in fluorescence exclusively localized to the synaptic terminal, with no detectable changes in either the axon or the soma. B, In the synaptic terminal, the percent of change in OG1 fluorescence increased with pulse duration. C, Pooled data (4-10 cells) on the relationship between the peak percent of change in fluorescence at synaptic terminals and the duration of the depolarizing pulse for experiments performed with 50 µM OG1. Note that the responses obtained with this high-affinity indicator saturate for pulses >50 msec. In contrast, as shown in D, the low-affinity indicator OG5 (200 µM) responds linearly throughout the duration range studied (pooled data from 5-17 cells). In C and D, error bars indicate SEM.

Because the use of low-affinity dyes could hinder the detection of minor changes in [Ca²⁺]_i in the axon and soma, the high-affinity Ca²⁺ indicator OG1 (K_d, ~170 nM according to Molecular Probes) was used. This dye could theoretically enable the detection of changes in [Ca²⁺]_i that would otherwise have been too small to be reported by OG5. OG1 was used only at a low concentration (50 µM) to minimize the effect of adding such a high-affinity Ca²⁺ buffer. This indicator proved to be sensitive to changes in fluorescence in terminals evoked by 5 msec depolarizing pulses. Pulses of durations ranging from 5 to 250 msec that led to clear increases in terminal F/F_o failed to produce any detectable changes in the axon and soma, however. Figure 7A presents an example with a 50 msec pulse (note that measurements in the dendrites could not be performed because of the out-of-focus contaminating fluorescence contributed by the pipette). In this set of experiments, faster time resolution (one image every 13 msec) was achieved by pixel binning (see Materials and Methods). For short-duration pulses (5-50 msec), both I_Ca and [Ca²⁺]_i transients peaked at the end of the pulse, and the relationship between peak F/F_o and pulse duration was linear (Fig. 7B) as with OG5 (Fig. 7, compare C,D, pooled data for OG1 and OG5). For longer depolarizations, however, fluorescence signals detected with OG1 saturated (Fig. 7C). In six cells, the decay time to 50% of peak F/F_o for 25 msec pulses was rather variable, ranging from 0.6 to >1.2 sec, the time at which data collection was stopped. These values were consistently larger than those measured for 50 msec pulses with OG5, in accord with previous comparisons of the time course of [Ca²⁺]_i transients in synaptic terminals using low- and high-affinity Ca²⁺ indicators (Regehr and Atluri, 1995; DiGregorio and Vergara, 1997; Helmchen et al., 1997; Sinha et al., 1997).

[Ca²⁺]_i rises restricted to terminals are specific to RBCs

Further support for a presynaptic locus for the sites of Ca²⁺ entry was derived from recordings obtained in neurons lacking synaptic terminals. Occasionally, bipolar cells having normal-looking somata and axons but lacking presynaptic boutons were encountered, probably because the axon was cut during the slicing procedure. Figure 8Aa shows an image taken after recordings had been performed in two cells, the somata of which were located in the INL. One of the cells has a clear synaptic bouton (and a normal I_Ca was recorded from it), whereas the other (upper quadrant of Fig. 8Aa) has an axon that descends toward the ganglion cell layer but lacks a synaptic terminal. This cell had passive properties similar to those of RBCs, but it did not show inward currents in response to depolarizations (Fig. 8Ab). In such cells no fluorescence transients were observed either at the soma or at the axon (data not shown).

View larger version (39K): [in this window] [in a new window]   Figure 8.   A, Lack of ICa in RBCs lacking terminals. Aa, Photomontage of an area of a retinal slice in which two bipolar cells were recorded; the top cell (with the pipette attached to its soma) lacks part of the axon and the terminal, and depolarizing pulses to 20 mV from a Vh of 70 mV failed to elicit ICa (Ab). Internal solution was CsGlu. B, ICa and [Ca2+]i rises in CBCs. Ba, Photomontage from OG5 fluorescence images showing a CBC with numerous synaptic terminals. Bb, The ICa elicited in this cell (internal solution was CsGlu) by 250 msec depolarizing pulses to 30 mV from a Vh of 70 mV shows pronounced inactivation. Bc, Bd, Depolarization-evoked change in fluorescence were not only observed in the bipolar terminals but also in the enlarged regions of the axon. No changes were detected in the soma. Internal solution was CsGlu (200 µM OG5, no EGTA). Photomontages in Aa and Ba were constructed from images taken at the end of the experiments, as detailed in Materials and Methods. Arrows indicate the approximate boundaries of the different layers identified under transmitted illumination. INL, Inner nuclear layer; IPL, inner plexiform layer; GCL, ganglion cell layer.

Although the present study focuses on RBCs, we searched for CBCs to compare their [Ca²⁺]_i signaling with that of RBCs. Despite the fact that 50% of the bipolar cells in the rat retina are cone bipolars (Euler and Wässle, 1995), the probability of recording from a CBC was extremely low in the present study. Of 72 bipolar cells recorded, only four were CBCs (6%) according to the stratification level of their axon, the branching pattern, and the presence of multiple synaptic terminals (Euler and Wässle, 1995). Three of these cells exhibited inactivating I_Ca, whereas one had L-type I_Ca. [Ca²⁺]_i dynamics were clearly different from those of RBCs. Figure 8B shows an experiment from one of these cells. The branching pattern and stratification of the axon in the IPL (Fig. 8Ba) suggests that this cell is a cone bipolar, presumably of type 6, 7, or 8 as described by Euler and Wässle (1995). With a CsGlu internal solution, depolarization to the maximal activation voltage for I_Ca elicited strongly inactivating inward currents (Fig. 8Bb) that were considerably larger than the average found for RBCs. [Ca²⁺]_i rises were detected in all synaptic boutons and the proximal axon, but not in the soma (Fig. 8Bc). The changes in axonal [Ca²⁺]_i had a slower rise time than those at synaptic boutons, and their magnitude decreased with the distance from the boutons. It is thus possible that axonal [Ca²⁺]_i rises in CBCs result largely from diffusion of Ca²⁺ from the terminals. Whether this explanation holds true, the spatial profile of [Ca²⁺]_i rises is strikingly different from that obtained for RBCs.

	DISCUSSION

Top Abstract Introduction Materials & Methods Results Discussion References

We show that in mammalian retinal slices, not only are somatic recordings feasible, but terminal patch-clamp recording is also possible from RBCs. The relatively large presynaptic structure of RBCs allowed us to compare the I_Ca obtained through direct terminal recordings with that measured via somatic recordings. Further experiments will unveil whether capacitance measurements can be achieved to provide information about the exocytotic and endocytotic processes.

Ca²⁺ currents in RBCs are mediated by HVA L-type calcium channels

In this study we have shown that RBCs possess HVA Ca²⁺ channels, the activation of which gives rise to highly localized [Ca²⁺]_i rises in the presynaptic terminals. We found a complete absence of a transient I_Ca but found the presence of an HVA calcium current that inactivates very slowly and is sensitive to DHP antagonists and agonists. This evidence thereby points to the L-type Ca²⁺ channel as mediating this current. In contrast, three of four recordings from CBCs exhibited pronounced inactivation for I_Ca. In isolated mouse bipolar cells, T-type channels have been reported to mediate Ca²⁺ influx; I_Ca inactivates rapidly, and it is insensitive to both DHP agonists and antagonists, as well as to low Cd²⁺ concentrations (Kaneko et al., 1989). Recently, a study of mouse bipolar cells in slices ascertained the additional presence of a DHP-sensitive component of I_Ca (de la Villa et al., 1998). Neither of these studies attempted to identify the cell type (rod vs cone) recorded, however. It is worth noting that there are at least nine types of CBCs in the rat retina (Euler and Wässle, 1995). Heterogeneity on the distribution of Ca²⁺ channel types among CBCs might explain the apparent discrepancies between our results and those obtained from mice.

Our results are in agreement with those of Pan and Lipton (1995), who reported that L-type Ca²⁺ channels mediate the [Ca²⁺]_i rises induced by K⁺ depolarization in the presynaptic terminals of isolated rat bipolar cells. Moreover, the combined application of voltage-clamp and imaging techniques to RBCs in slices strengthens the evidence that L-type calcium channels are the permeability pathway for Ca²⁺ ions in this cell type.

Terminal recordings support a preferential localization of Ca²⁺ channels in presynaptic terminals

The amplitude, inactivation kinetics, and pharmacological properties of I_Ca in RBCs were closely similar for recordings obtained from the soma and the presynaptic terminals. In terminal recordings, however, the I-V relationship was slightly shifted to the right of the voltage axis (both activation threshold and peak), and no escape of voltage clamp was observed in the presence of Bay K, indicating a more accurate membrane voltage control. A similar distinction for somatic and terminal recordings has been observed in goldfish Mb1 cells. A shift to the right of ~8 mV for activation threshold and ~12 mV for the peak of I_Ca was detected when comparing somatic with terminal recordings (Mennerick et al., 1997). Mennerick et al. (1997) modeled these cells as two compartments, soma and terminal (the latter possessing almost the totality of the Ca²⁺ channels), bridged by the axonal axial resistance, and found similar shifts in I_Ca kinetics when simulating recordings with a pipette placed either at the terminal or at the soma, consistent with our experimental observations.

Our finding that presynaptic L-type Ca²⁺ channels mediate the Ca²⁺ influx responsible for neurotransmitter release in mammalian RBCs is in agreement with the role of this channel type in other neurons that release neurotransmitter in a graded manner. A similar function has been ascribed to L-type Ca²⁺ channels in Mb1 bipolar cells (Tachibana et al., 1993; Heidelberger et al., 1994; von Gersdorff and Matthews, 1994; Sakaba et al., 1997), mammalian outer hair cells (Nakagawa et al., 1991), salamander rods (Corey et al., 1984), and lizard cones (Maricq and Korenbrot, 1988). The slow inactivation rate of these L-type currents differs from that in myocytes (Hadley and Lederer, 1991) and hippocampal neurons (Köhr and Mody, 1991) in which I_Ca inactivates in the tens of milliseconds range. It is similar to that of I_Ca in goldfish bipolar terminals (von Gersdorff and Matthews, 1996) in which both a tonic and a phasic mode of exocytosis (Mennerick and Matthews, 1996; von Gersdorff and Matthews, 1997) and subsequent neurotransmitter release occur (Tachibana et al., 1993; Sakaba et al., 1997). Thus, slowly inactivating L-type Ca²⁺ channels seem to be more adequate for synapses that must handle both phasic and graded signal transmission (Juusola et al., 1996) rather than N or P/Q subtypes that inactivate more rapidly and operate at synapses with strictly transient transmission such as the calyces of Held (Takahashi et al., 1996), the chick ciliary ganglion (Stanley and Goping, 1991; Yawo and Momiyama, 1993), and other CNS synapses (Dunlap et al., 1995).

Inhibitory negative feedback

A remarkable characteristic in some of our recordings was the presence of transient outward currents superimposed on the inward Ca²⁺ fluxes elicited by depolarization. The low-chloride internal solution used in our experiments resembles the physiological ionic composition; in these conditions, outward currents carried by Cl would lead to a hyperpolarization, which would, in turn, shut down the Ca²⁺ conductance and transform a sustained response into a transient one, consistent with the reported light responses in rabbit RBCs (Raviola and Dacheux, 1987). The sensitivity of these outward currents to GABA_A, GABA_C, and glycine antagonists indicates that they arise from reciprocal feedback synapses. Morphological studies have established that RBCs make a dyad synapse in the IPL onto both GABAergic A17 amacrine cells and glycinergic AII amacrine cells (Kidd, 1962; Dowling and Boycott, 1966; Wässle and Boycott, 1991). It has been shown that both cell types contain synaptic vesicles in the dendritic processes facing the rod bipolar endings with a higher vesicle density in the A17 (Raviola and Dacheux, 1987).

Furthermore, the presence of both GABA and glycine receptors in the synaptic terminals of mammalian RBCs has been largely demonstrated. Both neurotransmitters applied locally to the axonal endings elicit bicuculline-, picrotoxin-, and strychnine-sensitive Cl currents (Karschin and Wässle, 1990; Suzuki et al., 1990). Electrophysiological studies have shown that RBCs express GABA_A and GABA_C receptors (Feigenspan et al., 1993), and the presence of the GABA  subunit in these cells was further confirmed by the combined use of patch-clamp recordings with single cell RT-PCR (Yeh et al., 1996). Finally, GABA inhibits Ca²⁺ influx into RBC terminals via activation of GABA_A and GABA_C receptors (Pan and Lipton, 1995), and these two receptor types have been detected immunocytochemically in endings of rod bipolars (Greferath et al., 1995; Enz et al., 1996; Koulen et al., 1998). This combined evidence therefore supports the interpretation of our data that amacrine cells, via reciprocal feedback synapses on RBCs, are responsible for the outward current transients elicited by Ca²⁺ entry. Similar findings consistent with this hypothesis have been recently reported in abstract form (Hartveit, 1997). The low frequency of occurrence of such reciprocal synaptic currents in the present experiments is likely to result from disruption of synaptic connections during the slicing procedure at the slice surface where recordings were obtained.

Ca_i rises in RBCs are restricted to presynaptic terminals

The measurements with Ca²⁺ indicators confirm that Ca²⁺ influx in RBCs is restricted to the presynaptic terminals, with no detectable influx in the soma or axon. Along with the similarity in activation kinetics of I_Ca observed at the two recording sites, these findings suggest that RBCs possess a compact electrotonic structure that allows a passive spread of the voltage signal from the somatodendritic domain to the synaptic terminals where L-type Ca²⁺ channels are preferentially located to mediate tonic transmitter release.

The complete absence of [Ca²⁺]_i rises in RBC axons contrasts with findings in other central neurons. Imaging studies have shown that the large depolarization-evoked [Ca²⁺]_i rises occurring at synaptic varicosities in cortical neurons (Mackenzie et al., 1996) and cerebellar interneurons (Llano et al., 1997) are accompanied by smaller changes in [Ca²⁺]_i in the axonal regions between varicosities. These changes presumably originate from the redistribution of Ca²⁺ ions that takes place after a [Ca²⁺]_i rise. Furthermore, clear changes in [Ca²⁺]_i take place in the preterminal region of the calyces of Held (Borst et al., 1995), in the axon initial segment of neocortical pyramidal neurons (Schiller et al., 1995), and in the proximal axon of cerebellar Purkinje cells (Callewaert et al., 1996) after a single action potential. In our experiments, no detectable [Ca²⁺]_i rise was obtained in RBC axons at close distances to the terminals, even for rather long depolarizations. This finding suggests a highly effective system for Ca²⁺ removal, ensuring that Ca²⁺ ions are cleared from the axonal cytoplasm at a rate similar to that of Ca²⁺ diffusion into the axon. The axonal-terminal segregation of [Ca²⁺]_i rises seems to be particular to RBCs, because CBCs showed clear axonal Ca_i rises in response to depolarizations. Diffusion from the presynaptic boutons is likely to account for the axonal [Ca²⁺]_i signals, because they were delayed with respect to the terminal signals. It is worth noting, however, that the absence of axonal sites for Ca²⁺ influx deduced from the present work is not consistent with the presence of synaptic ribbons along the axons of several different types of CBCs, as well as in axons of RBCs in the cat retina (McGuire et al., 1984). Detailed exploration of bipolar cell axons at the electron microscopic level in the rat retina will be required to settle this issue.

	FOOTNOTES

Received Jan. 15, 1998; revised March 6, 1998; accepted March 6, 1998.

This work was supported by the Max-Planck-Society and a von Humboldt postdoctoral fellowship to D.A.P. We are grateful to A. Marty, H. von Gersdorff, and A. Boxall for their comments on this manuscript and C. Pouzat and C. Rosenmund for discussions.

Correspondence should be addressed to Dr. Isabel Llano, Arbeitsgruppe Zelluläre Neurobiologie, Max-Planck-Institut für biophysikalische Chemie, Am Fassberg, 37070 Göttingen, Germany.

Dr. Protti's present address: Abteilung Neuroanatomie, Max-Planck Institut für Hirnforschung, Deutschordenstrasse 46, D-60528 Frankfurt, Germany.

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