Ion-dependent Inactivation of Barium Current through L-type Calcium Channels

Abstract

It is widely believed that Ba²⁺ currents carried through L-type Ca²⁺ channels inactivate by a voltage- dependent mechanism similar to that described for other voltage-dependent channels. Studying ionic and gating currents of rabbit cardiac Ca²⁺ channels expressed in different subunit combinations in tsA201 cells, we found a phase of Ba²⁺ current decay with characteristics of ion-dependent inactivation. Upon a long duration (20 s) depolarizing pulse, I_Ba decayed as the sum of two exponentials. The slow phase (τ ≈ 6 s, 21°C) was parallel to a reduction of gating charge mobile at positive voltages, which was determined in the same cells. The fast phase of current decay (τ ≈ 600 ms), involving about 50% of total decay, was not accompanied by decrease of gating currents. Its amplitude depended on voltage with a characteristic U-shape, reflecting reduction of inactivation at positive voltages. When Na⁺ was used as the charge carrier, decay of ionic current followed a single exponential, of rate similar to that of the slow decay of Ba²⁺ current. The reduction of Ba²⁺ current during a depolarizing pulse was not due to changes in the concentration gradients driving ion movement, because Ba²⁺ entry during the pulse did not change the reversal potential for Ba²⁺. A simple model of Ca²⁺-dependent inactivation (Shirokov, R., R. Levis, N. Shirokova, and E. Ríos. 1993. J. Gen. Physiol. 102:1005–1030) robustly accounts for fast Ba²⁺ current decay assuming the affinity of the inactivation site on the α₁ subunit to be 100 times lower for Ba²⁺ than Ca²⁺.

introduction

Brief openings of L-type Ca²⁺ channels cause the increases in intracellular Ca²⁺ concentration required to effect rapid metabolic switching in a variety of cellular processes (Tsien and Tsien, 1990). The Ca²⁺ signalling process is controlled and limited by multi-layered inactivation mechanisms, that affect the plasmalemmal as well as the intracellular release Ca²⁺ channels. Channel inactivation sharpens the kinetics and temporal precision of the signals, and prevents longer term increases in [Ca²⁺]_i, which, among other problems, lead to stimulation of intracellular proteolysis (Turner et al., 1988).

In L-type and other Ca²⁺ channels (Tareilus et al., 1994; Cox and Dunlap, 1994), inactivation is produced by two mechanisms. One is mediated by the calcium ions that carry the current (Brehm and Eckert, 1978; Eckert and Chad, 1984), and it appears to involve binding to a site highly specific for Ca²⁺. In L-type channels the site is located near the channel mouth (Imredy and Yue, 1992, 1994; Shirokov et al., 1993), on the main (α₁) channel protein (Neely et al., 1994), and has been equated with an EF hand-like portion of the cytoplasmic COOH terminus (De León et al., 1995).

The other mechanism of inactivation does not require the passage of current (Fox, 1981). It is linked to the change in transmembrane potential, and is accompanied by changes in gating currents, which are broadly termed inactivation of charge (Shirokov et al., 1992). The two mechanisms function independently, as demonstrated by the fact that changes in [Ca²⁺]_i (Hadley and Lederer, 1991) and Ca²⁺ current through the channels (Shirokov et al., 1993) do not affect gating currents.

Parallel recording of gating currents and ion currents helped elucidate voltage-dependent aspects of Ca²⁺ channel gating (Field et al., 1988; Bean and Ríos, 1989; Hadley and Lederer, 1989) but is complicated in native cells by the presence of substantial Na⁺ channel gating current. The present work overcomes this problem using tsA201 cells, an expression system virtually free of endogenous channels. With Ba²⁺ as the permeant ion, we compared inactivation of gating charge with decay of ion currents, under the prevailing hypothesis that inactivation of L-type channel current is exclusively voltage-dependent in the absence of Ca²⁺ (e.g., Kass and Sanguinetti, 1984). The results disproved this hypothesis, favoring instead a dual mechanism of inactivation.

methods

Preparation of Transfected and Native Cells

Experiments were performed in the large T antigen–transformed human embryonic kidney cells (tsA201 line) grown in DME medium (Sigma Chemical Co., St. Louis, MO) supplemented with 10% FBS (BioWhittaker, Walkersville, MD) and 1% penicillin/ streptomycin (Sigma) in 5% CO₂. Cardiac rabbit α_1C, rat brain β_2a, and rabbit skeletal muscle α₂δ cDNAs were cloned in pCR3, pCMV, and pMT2 plasmid vectors respectively. High purity (A₂₆₀/A₂₈₀ ≥ 1.95) large-scale plasmid preparations were obtained using standard protocols (Qiagen Inc., Chadworth, CA). Transfections were done with 30 μg of each expression plasmid in different combinations (α_1C, α_1C + β_2a, and α_1C + β_2a + α₂δ) using a modified calcium phosphate precipitation method (Chien et al., 1995) in 100-mm tissue culture dishes. Cells were incubated with DNA for 6–8 h and then were shocked with 10% DMSO for 8 min. After the shock, cells were transferred onto glass coverslips, fed with fresh media and incubated until further evaluation. Electrophysiological recordings were made within 24–48 h post-transfection on round nonclustered cells. No sizable ionic or gating currents were observed in tsA201 cells in the absence of transfection. After transfection, the fraction of cells selected and patched that had Ca²⁺ currents was 60–80%. Recording of native Ca²⁺ currents was carried out in single rabbit cardiac ventricular myocytes, which were obtained by an enzymatic dissociation method (modified from Mitra and Morad, 1985) from young (1,500 g) male mutt rabbits.

Electrophysiological Recording

Cells were placed in small chambers (<200 μl) and perfused by continuous flow of external solutions. Records were obtained by a standard whole-cell patch clamp procedure using an Axopatch 200A amplifier and a 16-bit A/D-D/A converter card (HSDAS 16; Analogic Corp., Peabody, MA) under a 486 PC computer. Patch electrodes had resistances of 1.5–4 MΩ. Whole-cell capacitance, calculated as the area under a linear capacitive transient elicited by a −10 mV pulse, was 6–40 pF. Capacitance and resistance compensations were routinely done, and the charging time constant was typically 100 μs. Ionic currents were sampled at 0.15–1 kHz and gating currents at 10–40 kHz, depending on pulse duration.

All the currents represented are asymmetric, obtained after subtraction of scaled control currents, and not corrected for baselines. The control currents were elicited by pulses from −90 to −110 mV before each depolarization and after holding the cell at −90 mV for 30 s. All experiments were carried out at room temperature (∼20°C).

Exponential Fitting and Statistics

Data are presented as averages ± SEM. Signficance of differences between mean values was evaluated by Student's t test. Time course of current decay was fitted (using a nonlinear least-squares routine) by the function Y₁ = b + a exp (−t/τ) or the function Y₂ = b + a _slow exp (−t/τ_slow) + a _fast exp (−t/τ_fast). A _fast, A _slow, and B are the best fit amplitude parameters, a _fast, a _slow, and b, normalized to their sum. A and B symbolize the normalized amplitudes in the single exponential fit. In all cases in which both fits converged, the statistical significance of the fit improvement provided by the two- exponential function Y₂ was evaluated. The test was based on the likelihood ratio statistic, LRS = (ssr ₁ − ssr ₂)/σ² (Hoel, 1971; Hui and Chandler, 1990), in which ssr ₁ and ssr ₂ are the sums of squares of the residuals for the two fits and σ² is the variance of the record. LRS has a χ² distribution with 2 degrees of freedom (the difference between the number of free parameters of Y₂ and Y₁). If the statistic exceeds 6.0, the improvement in fit provided by the two-exponential function is significant to better than 5%. σ² was estimated by ssr ₂/(N − 5), which, being probably in excess, gave an underestimate of LRS.

Solutions

The internal solution contained (in mM): 150 CsOH (or NMG), 110 glutamate, 20 HCl, 10 HEPES, 5 MgATP, and 10 EGTA (pH adjusted to 7.6 by addition of CsOH). Osmolality of the internal solution was routinely measured and adjusted to 300–320 mosmole/kg.

External recording solutions contained (in mM): 160 TEA-Cl, 10 Tris, and either 10 CaCl₂ or 10 BaCl₂. Sodium external solution contained (in mM): 150 NaCl, 10 HEPES. In some experiments about 0.5 μM CaCl₂ was added to this solution to stabilize the patch seal. In gating current experiments, 10–20 μM GdCl₃ was added to the external solution with 10 mM Ca²⁺. All external solutions were adjusted to pH 7.2 and 300–320 mosmole/kg.

results

Inactivation of Ba²⁺ Currents Had Two Distinct Kinetic Phases

The lack of substantial endogenous voltage-dependent ion currents in tsA201 cells allowed us to study the time course of decay of Ba²⁺ currents (I_Ba) during very long pulses (up to 40 s). Ca²⁺ and Ba²⁺ currents in a cell transfected with α_1C and β_2a cDNAs are illustrated in Fig. 1, A and B. As shown in panel B, and as described often for I_Ca, the time course of I_Ba decay was well fitted by a sum of two exponentials plus a constant (Y₂ in methods). The record and the best fit line are shown to overlap in the inset, where they are plotted semilogarithmically. The single exponential fit (dashed line) was poor.

Figure 1.

Kinetics of Ca²⁺ and Ba²⁺ currents. (A) Ca²⁺ currents elicited by depolarizing pulses of 16.5-s duration, from a holding potential of −90 mV to voltages indicated near the traces in mV. (inset) The current at +20 mV, normalized to peak value and plotted in semilog scale. (B) Ba²⁺ currents elicited by 16.5-s pulses. At membrane voltages from −20 to +60 mV I_Ba had a bi-exponential time course of decay. (inset) Semilog plot of I_Ba at +20 mV, normalized to its peak value. A sum of two exponentials fitted to I_Ba(t) is represented by a continuous line superimposed to the data. The dashed line represents the best fit single exponential. The LRS (defined in methods) was 354.3, indicating significant improvement by the two-exponential fit. (C) Parameters, defined in methods, of the two-exponential fit to I_Ba(t), (n = 19).

Families of records from 33 cells were fitted with one and two-exponential functions. At voltages positive to +20 mV, 12 cells were discarded because they had a small outward steady current. Two other cells, which had unusually slow activation kinetics, were discarded because the two-exponential fit was not significantly better than the single exponential fit, as judged by the LRS. The averages of parameters obtained from the remaining 19 cells are in Fig. 1 C. On average, the time constant of the fast component of I_Ba decay (τ_fast) was minimal at +20 to +40 mV and increased (at a P < 0.08) at +60 mV. The amplitudes of the two exponentials (A _slow and A _fast) were comparable. A _fast went through a maximum at +20 mV, decaying at higher voltages. The slow component became faster and its amplitude greater at increasing depolarization. B decreased from 0.3 at −20 mV to 0.05 at +20 mV and increased to 0.15 at higher voltages. Because in the selected cells there was little if any outward current, even after 40 s pulses to +40 mV, and because neither current rundown nor substitution of NMG⁺ for intracellular Cs⁺ affected the decay parameters, these appear to represent kinetics of the expressed channels. The crisp separation of the two decay phases and the observed differences in the dependencies of their parameters on voltage suggest the presence of two independent mechanisms of inactivation.

Only the Slow Phase of I_Ba Decay Was Accompanied by Reduction of Gating Charge

Using ionic current-blocking solutions we studied the effects of prolonged depolarization on the availability of gating currents associated with channel opening. The asymmetric (ON) charge transferred after the depolarizing transition of a 0.1 s pulse was equal to the (OFF) charge transferred upon repolarization. As expected from studies in native cells, prolonged depolarization reduced gating currents. This was demonstrated with one- and two-pulse protocols, to rule out errors due to ionic currents or fast recovery from inactivation of gating charge. Fig. 2 A shows the OFF transients obtained upon repolarization from +20 mV, after periods of depolarization indicated near the traces. The larger transient in each pair is the reference OFF after a 45-ms pulse (in every case preceding the prolonged depolarization). Surprisingly, reduction of charge transfer took much more time than decay of I_Ba. Fig. 2 B plots reduction of the OFF charge vs. pulse duration, averaged in nine cells. The curve is a single exponential fit (τ ≈ 8 s).

Figure 2.

Reduction of mobile charge takes seconds. (A) OFF gating current transients after increasing times at +20 mV. The records are asymmetric currents obtained as described in methods. Durations of the test depolarizations that preceded the transients are listed near each plot. Test OFF transients are shown superimposed with larger reference transients, obtained at the trailing edge of 0.045-s pulses applied before each test depolarization. (B) Difference between reference and test OFF charge transfer, normalized to reference, vs. duration of depolarization at +20 mV (n = 9). The continuous line represents ΔQ _max(1 − exp(−t/τ)), with ΔQ _max = 0.34 and τ = 8.7 s. (C) Gating currents elicited by a fixed test pulse after conditioning depolarizations of different durations (listed near each record). At left in the panel are the asymmetric currents during the conditioning depolarization, recorded at a slower sampling rate (up to the time indicated by the dotted line). Records obtained with and without conditioning pulse are shown superimposed. (D) Difference in ON charge transfer, reference minus conditioned, normalized to reference, vs. duration of the conditioning depolarization (open symbols, averages; n = 4; filled symbols, data from records in C). Continuous line generated as in B, with ΔQ _max = 0.49 and τ = 8.5 s.

The reduction of the available charge after depolarization was also monitored by a double pulse protocol illustrated at top of Fig. 2 C. The membrane was conditioned at +20 mV, then it was repolarized to −60 mV for 7 ms and a test pulse to +50 mV was applied to move the charge available at voltages of channel opening. During conditioning depolarization currents were recorded at a low acquisition rate, which was increased at the repolarization swing. As in Fig. 2 A, the larger transient in each pair is the reference obtained before the corresponding conditioning pulse. The reduction in available charge is plotted vs. conditioning duration in 2 D. The reduction of gating charge at positive voltages had the same time course as the reduction of the OFF charge in the single pulse experiment.

Fig. 3 compares the time course of I_Ba decay and that of gating charge reduction. In the figure we superimposed data and fit of charge availability (from Fig. 2 B) on a record of I_Ba elicited by a 16.5 s depolarization. The exponential decay of charge availability (solid curve) has a time constant similar to that of the slow decay of I_Ba, suggesting that these are due to a slow inactivation mechanism, distinct and voltage-dependent. On the other hand, the figure clearly shows that about half of the decay of I_Ba occurred much more rapidly than the process causing charge reduction. Indeed, as shown in Fig. 2 A, ON and OFF charges remained equal in single pulses of up to 1 s, a time at which ionic current had inactivated by ∼40%.

Figure 3.

Slow inactivation of I_Ba and reduction of mobile charge had the same kinetics. Ba²⁺ current evoked by a 16.5-s pulse to +20 mV from a holding potential of −90 mV. Shown superimposed are the average values and fit (thick line) of charge reduction at +20 mV (same as in Fig. 2 B). Parameters of the two- exponential fit to the Ba²⁺ current (dotted line): A _fast = 0.38, τ_fast = 0.75 s, A _slow = 0.57, τ_slow = 6.68 s, B = 0.05.

Fast Decay of I_Ba Is a Current-dependent Process

Fast inactivation of I_Ba was studied with brief (0.3 s) test pulses to +20 mV, following a 2 s conditioning pulse to different voltages (which should cause fast inactivation almost exclusively) and a 1 s interpulse to −60 mV (to ensure the return of all intramembrane charge). Each pair of pulses was preceded by a single test pulse for reference, and the sets were applied at 1-min intervals. Reference and conditioned currents are shown in pairs in Fig. 4 A, normalized to correct for rundown. A conditioning pulse to 0 mV (eliciting substantial I_Ba) reduced the magnitude and the rate of decay of the following test current. Conditioning at +80 mV evoked no inward current and had less effect on the test current. Averages in seven cells are plotted vs. conditioning voltage in Fig. 4 B. Circles represent peak conditioning current relative to the maximal value at +10 mV and squares represent peak test current (measuring channel availability after conditioning). I_Ba appeared at −30 mV, peaked at +10 mV, and decayed at higher voltages. The availability had a U-shaped voltage dependence that mimicked the voltage dependence of the conditioning current, as befits a current- (rather than voltage-) dependent inactivation process (Tillotson, 1979). This inactivation was not due to Ca²⁺ contamination, as [Ca²⁺] was measured in the external solutions with a Ca²⁺ electrode and found to be negligible (<5 μM).

Figure 4.

Availability of Ba²⁺ current after a brief conditioning pulse. (A) I_Ba elicited by a fixed test pulse after 2-s long conditioning pulses to different voltages (indicated in mV). Conditioned and reference current traces are shown superimposed. Within each pair, the currents are scaled to the peak of the reference current. Note symbols indicating measurements plotted in B. (B) Squares: peak of test I_Ba vs. conditioning voltage, (n = 7). Triangles : extent of inactivation of I_Ba during the test pulse, measured as (I_peak − I (300 ms))/I_peak, (n = 7). Circles : peak Ba²⁺ current during a pulse to the voltage in the abscissa, normalized in each cell to the maximum current (n = 19).

A U-shaped voltage dependence of the current availability could also be a manifestation of potentiation of channel activity by large positive pulses, as shown in snail neurons (Heyer and Lux, 1976), chromaffin cells (Hoshi et al., 1984), skeletal muscle (Sculptoreanu et al., 1993) and cardiac cells (Lee, 1987). However, the extent of current decay during the test pulses (triangles in Fig. 4 B) was minimal after conditioning at +10 mV and increased at more positive conditioning voltages. This implies that conditioning to a high voltage had a modest accelerating effect on the decay kinetics, which is against a major role of voltage-dependent potentiation, because in native cardiomyocytes potentiated currents had a much slower rate of decay (Lee, 1987). Also against voltage-dependent potentiation is the observation that the conditioned Ba²⁺ currents were never greater than reference currents, even after conditioning to +100 mV.

Fast Current Decay Was Absent when Na⁺ Was the Permeant Ion

Fig. 5 shows representative records of Na⁺ current (I_Na) through the α_1C/β_2a channels at submicromolar concentrations of extracellular divalent cations. The voltage dependence of I_Na (diamonds in Fig. 5 B) and its sensitivity to Ca²⁺ channel blockers were as described in native channels (Kostyuk et al., 1983; Hess et al., 1986), which proves that I_Na passed through the expressed L-type channels. In agreement with previous reports in isolated cardiac myocytes (Imoto et al., 1985; Hadley and Hume, 1987), I_Na activated at potentials about 30 mV more negative than I_Ba (circles). At all voltages I_Na decayed much more slowly than I_Ba. A scaled I_Ba trace plotted together with I_Na (Fig. 5 C) illustrates that the fast decay was absent when Ba²⁺ was removed. In fact, a fast component of decay was not resolvable even at very high densities of Na⁺ current (up to 54 A/F). Including Ca²⁺ in the external solution at a concentration of 20 μM led to the appearance of a phase of I_Na decay with kinetics similar to those of the fast inactivation of I_Ba (Fig. 5 C).

Figure 5.

The fast component of inactivation was absent when Na⁺ was the charge carrier. (A) Currents elicited in a Ca²⁺-free, 150 mM Na⁺ external solution by 16.5-s pulses to the voltages indicated in mV. (B) Diamonds: peak Na⁺ current, normalized to its maximum in each cell, vs. pulse voltage (n = 5). Circles : peak current in 10 mM Ba²⁺ (n = 19). Peak I_Na was 25.6 ± 4.3 A/F, whereas peak I_Ba was 36 ± 3.5 A/F. (C) Currents obtained in different cells, in either 150 mM Na⁺, 10 mM Ba²⁺, or 150 mM Na⁺ plus 20 μM Ca²⁺, at the voltages of maximal currents. Records were scaled to the same amplitude. Parameters of a single exponential fit to the Na⁺ current shown: A = 0.62, τ = 8.72 s, B = 0.38; two-exponential fits to Na⁺ + 20 μM Ca²⁺: A _fast = 0.43; τ_fast = 0.35 s, A _slow = 0.47, τ_slow = 5.84 s, B = 0.10; to Ba²⁺ current: A _fast = 0.46; τ_fast = 0.93 s, A _slow = 0.42, τ_slow = 12.63 s, B = 0.12. Note that the parameter values of the Na⁺ + 20 μM Ca²⁺ fit are not significantly different from the average values for I_Ba in α₁/β cells (Table I).

Absence of Bulk Accumulation Effects

It is believed that the level of Ca²⁺ accumulation produced by typical membrane Ca²⁺ currents cannot significantly change the driving force that determines Ca²⁺ flux in a cell buffered with several mM of EGTA (Neher, 1986). The buffering capacity of such intracellular solutions will be lower for Ba²⁺ (because the affinity of EGTA for Ba²⁺ is about 100 times less than for Ca²⁺; Harafuji and Ogawa, 1980). It is therefore conceivable that the current dependent reduction of I_Ba is due to a reduction of driving force on the ion upon accumulation of Ba²⁺ inside the cell. A simple single pool model of accumulation of Ba²⁺ in the volume of the cell, in which unidirectional Ba²⁺ fluxes are assumed to be independent, predicts first order decay of current, with rate constant proportional to initial current amplitude and to the reciprocal of cell volume. The volume of round cells (a good approximation for transfected tsA201 cells) is proportional to C_m ^3/2, where C_m is membrane capacitance. Fig. 6 A plots τ_fast ⁻¹ vs. (peak I_Ba/ C_m ^3/2) at +20 mV for 21 cells, demonstrating no correlation between these variables.

Figure 6.

Two tests of Ba²⁺ accumulation. (A) Rate constant of fast decay of Ba²⁺ currents elicited at different voltages in different cells vs. the ratio (peak I_Ba/C_m ^3/2). The correlation coefficient was r = 0.022. (B) I_Ba elicited by a test pulse to the reversal potential (+65 mV), following a 2-s conditioning pulse that elicited maximal I_Ba. The conditioned current is shown superimposed to the reference current, elicited without conditioning. Conditioned and reference currents were both nil during the test pulse.

The above test does not rule out depletion of Ba²⁺ ions outside the cell, or their accumulation in restricted spaces close to the conduction pathway. To test these possibilities we sought to demonstrate changes in the driving force for I_Ba, in experiments similar to those described in a study of Na⁺ accumulation (Hadley and Hume, 1987) and illustrated in Fig. 6 B. I_Ba was elicited with a double pulse protocol similar to that in Fig. 4. The test pulse took the membrane to the reversal potential and elicited no net ionic current. If a large current preceding the test determined substantial accumulation and a change in driving force for Ba²⁺, the conditioned pulse should elicit an outward current. Conditioning at 0 mV elicited near maximal I_Ba but did not result in the appearance of outward current during the test pulse. The decay in current can therefore be safely attributed to channel gating (inactivation) rather than a change in driving force.

Fast Decay Was Not due to Acidification

Ca²⁺ channel activity decreases at low intracellular pH (Kaibara and Kameyama, 1988) and EGTA is deprotonated when it chelates metal cations, with consequent acidification (Jong et al., 1993). Therefore, one possible mechanism of fast inactivation was channel closure due to acidification. Against this possibility we found that the fast phase of decay was present even when intracellular pH was buffered with 100 mM HEPES (data not shown). We also compared rates of I_Ba decay in cells dialyzed with 0.5, 1, 10, or 20 mM of EGTA. The rapidly decaying component was present in all and its kinetics changed only slightly (data not shown). These observations again rule out accumulation, as well as other possible mechanisms involving EGTA in the development of fast current decay.

Fast Inactivation of I_Ba Is a Property of the α₁ Subunit

To test whether fast inactivation depended on certain auxiliary subunits or other properties of the expression system, experiments were carried out with different combinations of subunits α_1C, β_2a, and α₂δ, and with native rabbit ventricular myocytes. As illustrated in Fig. 7, both phases of I_Ba decay were present in all cases, including cells transfected with α₁ alone. The parameters of two-exponential fits and their averages are listed in Table I.

Figure 7.

Kinetics of I_Ba with different combinations of subunits and in ventricular myocytes. Ba²⁺ currents elicited by 16.5-s pulses to +20 mV, in tsA201 cells transfected with cDNA combinations listed in each panel, and in a rabbit ventricular myocyte (native).

Table I.

Composition		Number of cells		A fast		A slow		B		τfast, (s)		τslow, (s)
α1C		6		0.35 ± 0.05		0.45 ± 0.03		0.20 ± 0.03		0.57 ± 0.06		6.88 ± 0.66
α1C/β2a		19		0.54 ± 0.04		0.39 ± 0.04		0.07 ± 0.02		0.65 ± 0.07		6.21 ± 0.81
α1C/β2a/α2δ		16		0.58 ± 0.04		0.37 ± 0.03		0.05 ± 0.03		0.58 ± 0.06		5.15 ± 0.55
native		3		0.67 ± 0.06		0.28 ± 0.04		0.04 ± 0.01		0.21 ± 0.01		1.78 ± 0.18

Two-exponential fits to I_Ba decay in tsA201 cells transfected with different combinations of L-type Ca²⁺ channel subunits, and in rabbit ventricular myocytes. I_Ba was elicited by 16.5-s long pulse from the holding potential of −90 mV to +20 mV. The fit function and parameters are described in methods. 

Although cells co-transfected with α_1C + β_2a had much higher current density than cells transfected with α_1C alone, the rates of inactivation were similar in both groups, consistent with the previous observation that β_2a, is the least potent among other cloned β subunits in acceleration of inactivation (De Waard and Campbell, 1995). A _fast increased significantly with the number of subunits, being maximal for the native channels. The kinetics of fast inactivation did not depend on the composition of the expressed channels, being in all cases about threefold slower than in native channels. The rate of the slow component increased with the number of subunits. This change was marginally significant between α_1C and α_1C/β_2a/α₂δ cells (at a level P < 0.09) and not significant between α_1C/β_2a and α_1C/β_2a/ α₂δ cells. (The histogram of slow time constants of the α_1C/β_2a/α₂δ cells was bimodal, with approximately one quarter of the α_1C/β_2a/α₂δ cells centered at about the same modal value as the α_1C/β_2a group. It is possible that a group of α_1C/β_2a/α₂δ cells expressed little of the α₂δ subunit or that the subunit did not incorporate stoi-chiometrically to the complex [Gurnett et al., 1996]. Therefore, the α₂δ subunit may have had a greater effect than that reflected by our averaged measurements.)

The presence of both decay phases with every combination of subunits indicates that both inactivation mechanisms are determined by the α_1C subunit. That the relative amplitudes and kinetics of the two phases varied with the subunit composition is consistent with a modulatory role of the auxiliary subunits (Catterall, 1995).

discussion

The present study was designed to compare inactivation of ionic and gating currents of L-type Ca²⁺ channels in the simplest possible situation. The tsA201 cells provided a system essentially devoid of other channels. Use of Ba²⁺ as current carrier was expected to eliminate the current-dependent inactivation mechanism. In spite of these conditions, inactivation of ionic current was found to follow two kinetic phases, of which only the slow one was co-temporal with the observed single exponential reduction of gating charge. The fast phase was current-dependent and did not correlate with the reduction of the gating charge. Because the two kinetic phases of inactivation of I_Ba were seen in cells transfected with the α_1C subunit, alone, in combination with β_2a or with β_2a and α₂δ, as well as in rabbit ventricular myocytes, they must be a property of the α₁ subunit, depending on neither the auxiliary subunits nor the expression system. In this section we analyze the present findings, compare them with published observations and infer that the fast phase of decay is caused by Ba²⁺ binding to the channel's Ca²⁺-inactivation site.

The Population of Ca²⁺ Channels Was Homogeneous

Ba²⁺ currents through L-type Ca²⁺ channels have been observed to decay in two phases in many different preparations. In neurons, two components of decay were observed, but the significance of the observation was obscured by the existence of multiple types of high voltage-activated Ca²⁺ channels (Boland and Digledine, 1990; Kay, 1991). In cardiac myocytes, the presence of two components of inactivation of I_Ba was interpreted as due to two different processes of voltage-dependent inactivation, because inactivation of I_Ba was believed to be purely voltage dependent (Kass and Sanguinetti, 1984; Lee et al., 1985; Boyett et al., 1994). This view could not be tested rigorously because in cardiac myocytes it is difficult to correlate inactivation of I_Ba with inactivation of gating currents, due to the contribution of other channels to charge movement (Bean and Ríos, 1989; Shirokov et al., 1992). These problems may have been circumvented in the present work, provided that the Ca²⁺ channels expressed in a mammalian cell line after transfection were a single population, homogeneous in its biophysical properties. This seems to have been the case, for the three following reasons:

No sizable Ca²⁺ or Ba²⁺ currents were recorded in mock-transfected cells. In our experiments, amplitudes of endogenous currents (<0.5 A/F) were always one or two orders of magnitude smaller than those in transfected cells. Therefore, the bulk of the Ba²⁺ or Ca²⁺ current in transfected tsA201 cells was probably conducted through recombinant channels, and endogenous currents could not have been the reason for the multiplicity of inactivation phases.

In agreement with Kamp et al. (1996) and Josephson and Varadi (1996), we found a consistent correlation between the amount of intramembranous mobile charge and the ionic current density, suggesting that a major fraction of expressed channels function to carry current.

When rundown reduced ion current amplitude, the relative magnitudes of the two inactivation phases were conserved. Had the processes taken place in two different sets of channels, their proportions would not have been likely to remain constant during rundown.

Assuming that the population of channels was homogeneous, the question that then arises is if the kinetic phases of inactivation correspond to two different mechanisms.

Ba²⁺-dependent Inactivation Caused the Fast Decay of Current

The fast decay of current depended on the current through the channel, rather than the applied voltage. This was demonstrated by three observations:

In experiments with a double pulse protocol, current availability depended on the voltage of the conditioning pulse in a U-shaped manner, and inactivation reached a maximum at voltages that made inward current greatest, much as has been described for Ca²⁺-dependent inactivation (Eckert and Chad, 1984). In the present experiments the observation was free from many errors that may have obscured this property in previous studies with native cardiomyocytes. Although a U-shaped voltage dependence is expected in current-dependent processes, it could also arise from (voltage-dependent) potentiation, that offsets the inactivation effect at high voltages (Lee, 1987). Voltage-dependent potentiation cannot explain the present observations because current elicited by the test after a high voltage conditioning pulse was never greater than reference, and its kinetics remained the same. Our failure to observe voltage-dependent potentiation agrees with the report of Cens et al. (1996) that β_2a failed to promote voltage-dependent potentiation, at variance with the effects of other types of β subunit.

Recovery of I_Ba from inactivation was slower after a conditioning to +20 mV than to +60 mV (data not shown). Much more Ba²⁺ enters the cell during a pulse to +20 than at +60 mV. The longer lasting inactivation induced at +20 mV may simply be a consequence of the persistence of inactivating concentrations of Ba²⁺ near the channels for a longer time (as argued by Kay, 1991, for Ca²⁺ currents in neurons).

There was no immobilization or voltage shift of gating current with kinetics corresponding to those of the fast decay of ionic current. In the current view, inactivation of Na⁺ and K⁺ channels acquires its voltage dependence indirectly, through a link to channel opening. In Na⁺ and K⁺ channels inactivation is more likely to happen when gating particles are in the activating position. In a microscopically reversible system, this implies that inactivation stabilizes the voltage sensor in its activating position, negatively shifting the transition voltage of gating currents and reducing the availability of charge mobile in the range of voltages that normally cause activation. This was not found in our case for the fast component of inactivation of I_Ba.

The observed decay of I_Ba could not have been due to bulk accumulation or cell loading by the permeating Ba²⁺, as the effect failed to correlate with the geometry of the cell (Fig. 6 A), and Ba²⁺ entry during long-lasting depolarization failed to change the reversal potential of the current (Fig. 6 B). This conclusion is also consistent with the finding (Cavalié et al., 1983) that the amplitude of single channel current remains the same during prolonged depolarization. The decay can therefore be attributed to an inactivation gating process, dependent on the local increase of [Ba²⁺], at levels that do not significantly change the driving force for I_Ba.

The evidence strongly favors a mechanism that requires binding of Ba²⁺ to a site on the channel molecule. Most importantly, the fast decay of Ca²⁺ channel current was absent when Na⁺ carried the current, even at high current densities. This fact is further evidence against an accumulation phenomenon, which would not be expected to work solely for Ba²⁺. Furthermore, because I_Ba in α₁ cells exhibits the fast decay, the putative Ba²⁺ site has to be on the α₁ polypeptide. That the fast decay was observed in currents carried by Ba²⁺, by Ca²⁺, and by Na⁺ in the presence of extracellular Ca²⁺, suggests that Ba²⁺ causes inactivation by binding to the Ca²⁺-inactivation site. That fast inactivation of Ba²⁺ current occurred without correlative changes in gating current is consistent with this hypothesis, considering that the voltage-dependent and the Ca²⁺-dependent mechanisms of inactivation do not interact (Hadley and Lederer, 1991; Shirokov et al., 1993).

Previous work has failed to clarify whether or not I_Ba inactivates by an ion-dependent mechanism. McDonald et al. (1986) did not find U-shaped voltage dependence for inactivation of Ba²⁺ currents in on-cell patches of guinea pig ventricular myocytes. On the same preparation, Imredy and Yue (1994) saw some reduction in the extent of decay of single channel I_Ba at voltages above +20 mV, and tentatively interpreted it as evidence of Ba²⁺-dependent inactivation. Mazzanti et al. (1991) found fast decay of Ba²⁺ current provided that there were multiple channels in a patch, and proposed a Ba²⁺-dependent mechanism of inactivation enhanced by channel clustering. The interpretation of single channel on-cell measurements is complicated by the possibility of inactivation by Ca²⁺ released from intracellular stores (Galli et al., 1994; Sham et al., 1995). Schneider et al. (1991) found that entry of Ba²⁺ into smooth muscle cells through ATP-activated channels reduced whole-cell L-type channel Ba²⁺ currents by about 20%. Perfusion of rabbit portal vein smooth muscle cells with 100 μM of Ba²⁺ in the patch pipette led to a 10% reduction of I_Ca (Ohya et al., 1987). The results are consistent with a finding of Brown et al. (1981) that perfusion of Helix aspersa neurons with 1 mM Ba²⁺ in the pipette reduced I_Ba by some 20%. In sum, the evidence with single channels is inconclusive, while in whole cells there are modest effects of perfusion with Ba²⁺. These results do not rule out inactivation by the high concentrations of Ba²⁺ that are likely to occur at the putative site, which is presumably located near the channel mouth (De León et al., 1995).

The main characteristics of Ca²⁺-dependent inactivation of I_Ca were previously reproduced with a simple three-gate model of the L-type channel (Shirokov et al., 1993). We now show that this model also accounts for the properties of I_Ba, assuming that Ba²⁺ substitutes for Ca²⁺ at the inactivation site. The model includes voltage-dependent properties, activation, and inactivation, which are independent of cation binding, and are represented in scheme I:k_RI,RPk_RP,RIRIRPAIAPk_AP,AIk_AI,APk_AP,RPk_RP,AP (scheme I)k_AI,RIk_RI,AI

Activation is the opening of a voltage-operated gate, whose states are resting (R) and activated (A). Voltage-dependent inactivation involves a second gate, with a permissive (P) and an inactivated state (I). The P → I transition is not intrinsically voltage-dependent, but is favored from channel state AP.¹

Ion-dependent inactivation is pictured by a third gate, the states of which are represented in scheme II:

k_C,CMek_CMe,CC + Me²⁺C:Me²⁺U + Me²⁺U:Me²⁺k_UMe,Uk_U,UMek_{Ume, CMe}k_{CMe, UMe} (scheme II)k_u,ck_c,u

The ion-controlled gate can be “covering” (C, channel closed) or “uncovering” (U). Me²⁺, normally Ca²⁺, inactivates the channel because its binding stabilizes state C, that is, the equilibrium between C:Me²⁺ and U:Me²⁺ is shifted toward C:Me²⁺. Accordingly, and to satisfy microscopic reversibility, the affinity of the site must be greater in state C than in state U. The channel state is described by the state of its three gates and is open only in state APU.² The ion-dependent inactivation process does not affect the voltage-dependent processes in any way (implying that the evolution of states depicted in scheme I can be solved independently), while the states in scheme II are influenced by the voltage-dependent gates only because the concentration of the current-carrying ion changes when the channel opens. [Me²⁺] at the site was assumed to be an instantaneous function of the channel current i, defined as: [Me²⁺]_bulk + i/ 4πFDr, where [Me²⁺]_bulk is 50 nM, F is the faraday, the diffusion constant D is 10⁻⁶ cm²s⁻¹, and the distance r from the channel mouth to the binding site is 1 nm.

In this model, dissociation constants (K _d) for Ca²⁺ are supposed to be 1 μM in state C and 100 μM in state U. I_Ba was simulated assuming 100-fold higher K _ds in both states (which was achieved by reducing the binding rate constants). The only other difference between the two ions was a two-times greater single channel current for Ba²⁺ at any given extracellular [Me²⁺].³

The simulations⁴ are illustrated in Fig. 8, where current records, exponential fits, and fit parameters are shown in a manner similar to Fig. 1. With this choice of parameters the model reproduced well the main properties of I_Ba, including: the presence of two kinetic phases of inactivation, the voltage dependence of τ_slow, the amplitudes of all components, and the fact that τ_fast was steeply voltage-dependent for I_Ca (Fig. 8 A) but not I_Ba (Fig. 8 B).

Figure 8.

A model of Ca²⁺-dependent inactivation can also describe Ba²⁺currents. Simulations with the model described in the text, presented and analyzed in the same order as the experimental records in Fig. 1. (A) Simulated I_Ca elicited by pulses from −90 mV to voltages indicated near the traces. (inset) Simulated I_Ca at 0 mV, normalized to the peak value and plotted in semilog scale. (B) Simulated I_Ba during long duration pulses to voltages indicated. Dashed lines: two-exponential fits. (inset) Simulated I_Ba at 0 mV, normalized to the peak value and plotted in semilog scale. (C) Parameters of two-exponential fits to the simulated I_Ba.

Voltage-dependent Inactivation Underlies the Slow Phase of Current Decay

The present results include a reduction in the amount of charge available to move above −60 mV, upon prolonged depolarization. This reduction, which depends exponentially on duration of the depolarizing pulse, is cotemporal with the slow phase of current decay, regardless of the ion that carries the current. This implies that the slow phase of decay of I_Ba is the result of voltage-dependent inactivation. The concomitant reduction in the availability of gating charge could be the consequence of two not mutually exclusive mechanisms: charge immobilization associated with inactivation (Armstrong and Bezanilla, 1977), or a negative shift in the voltage distribution of intramembrane mobile charge, similar to that accompanying slow inactivation of squid Na⁺ channels (Bezanilla et al., 1982), inactivation of the voltage sensor of skeletal muscle (Brum et al., 1988), and inactivation of L-type channels in guinea pig cardiomyocytes (Shirokov et al., 1992) and embryonic chick ventricular myocytes (Josephson, 1996).

Implications for Other Ca²⁺ Channel Studies

The present results define two kinetic components of decay of Ba²⁺ currents through Ca²⁺ channels, show that the slow phase, with characteristic times of seconds, is caused by voltage-dependent inactivation, and suggest binding of Ba²⁺ as probable cause for the fast phase. These findings call into question the widespread use of Ba²⁺ currents as tools to quantify purely voltage- dependent processes in Ca²⁺ channels. By showing the close association between gating current inactivation and a decay of current that takes place in seconds, it forces reconsideration of studies that attribute decay phases of hundreds of ms to voltage-dependent processes.

For example, Zong et al. (1994), in their study of L-type Ca²⁺ channels in HEK 293 cells, used the difference between the “slow” time constant (∼200 ms) in a two- exponential fit to I_Ca elicited by 400-ms pulses, and the time constant in a single exponential fit to I_Ba (∼300 ms) to argue that Ca²⁺ may make voltage-dependent inactivation faster. Clearly the time constants were too short (and so were the applied pulses) to significantly explore the voltage-dependent process, which we now show to be much slower.

Zhang et al. (1994) analyzed the kinetics of I_Ba through chimeric channels in Xenopus oocytes to localize determinants of voltage-dependent inactivation. In this study, an α_1A (a putatively P/Q-type channel from brain) with relatively slow rate of I_Ba decay was chimerized with the rapidly inactivating α_1E (doe-1, marine ray). The work unquestionably localized the determinants of subunit-specific differences in decay of I_Ba to segment IS6 and its vicinity. Because the inactivation of I_Ba in doe-1 is believed to be exclusively voltage dependent (Ellinor et al., 1993), the rates of decay found in the rapidly inactivating chimeras, 10–30 s⁻¹, were naturally attributed to voltage-dependent inactivation. However, P-type channels are susceptible to Ca²⁺-dependent inactivation (Tareilus et al., 1994), and therefore the assertion that fast inactivation in the chimeras is voltage-dependent should be supported with the use of longer pulses or other tests.

Possible involvement of the first domain in determining the rate of I_Ba decay was also demonstrated by Parent et al. (1995) working with a chimera of α_1C and α_1S. Even though the demonstration was clear, the conclusion that the first repeat affects voltage-dependent inactivation can be criticized on similar grounds, because it relies on the assumption that I_Ba inactivation is exclusively voltage-dependent.

In conclusion, the identification of structural determinants of voltage-dependent inactivation in Ca²⁺ channels can not be based solely on the analysis of I_Ba, since the ability to induce inactivation of the L-type Ca²⁺ channel appears not to be a unique property of Ca²⁺ ions. The main consequence of the present work is to require careful reconsideration of the mechanisms attributed to inactivation in previous and future studies.