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The Journal of Neuroscience, May 1, 2002, 22(9):3645-3655

Upregulation of a T-Type Ca²⁺ Channel Causes a Long-Lasting Modification of Neuronal Firing Mode after Status Epilepticus

Hailing Su^{1, *}, Dmitry Sochivko^{3, *}, Albert Becker², Jian Chen³, Yanwen Jiang¹, Yoel Yaari¹, and Heinz Beck³

¹ Department of Physiology, Hebrew University-Hadassah School of Medicine, 91120 Jerusalem, Israel, and Departments of ² Neuropathology and ³ Epileptology, University of Bonn Medical Center, D-53105 Bonn, Germany

	ABSTRACT

TOP ABSTRACT INTRODUCTION MATERIALS AND METHODS RESULTS DISCUSSION REFERENCES

A single episode of status epilepticus (SE) causes numerous structural and functional changes in the brain that can lead to the development of a chronic epileptic condition. Most studies of this plasticity have focused on changes in excitatory and inhibitory synaptic properties. However, the intrinsic firing properties that shape the output of the neuron to a given synaptic input may also be persistently affected by SE. Thus, 54% of CA1 pyramidal cells, which normally fire in a regular mode, are persistently converted to a bursting mode after an episode of SE induced by the convulsant pilocarpine. In this model, intrinsic bursts evoked by threshold-straddling depolarizations, and their underlying spike afterdepolarizations (ADPs), were resistant to antagonists of N-, P/Q-, or L-type Ca²⁺ channels but were readily suppressed by low (30-100 µM) concentrations of Ni²⁺ known to block T- and R-type Ca²⁺ channels. The density of T-type Ca²⁺ currents, but not of other pharmacologically isolated Ca²⁺ current types, was upregulated in CA1 pyramidal neurons after SE. The augmented T-type currents were sensitive to Ni²⁺ in the same concentration range that blocked the novel intrinsic bursting in these neurons (IC₅₀ = 27 µM). These data suggest that SE may persistently convert regular firing cells to intrinsic bursters by selectively increasing the density of a Ni²⁺-sensitive T-type Ca²⁺ current. This nonsynaptic plasticity considerably amplifies the output of CA1 pyramidal neurons to synaptic inputs and most probably contributes to the development and expression of an epileptic condition after SE.

Key words: T-type Ca²⁺ channel; status epilepticus; intrinsic burst discharge; plasticity; CA1; hippocampus

	INTRODUCTION

TOP ABSTRACT INTRODUCTION MATERIALS AND METHODS RESULTS DISCUSSION REFERENCES

Both in humans and in experimental animals, continuous seizure activity as occurs during status epilepticus (SE) results in a large number of plastic changes within the hippocampus and adjacent brain areas (Coulter and DeLorenzo, 1999; Sloviter, 1999; Ben Ari, 2001). The SE-induced modifications in neuronal function may consist either of altered synaptic function or of changes in the intrinsic membrane properties of neurons. Hitherto, a multitude of structural and functional synaptic changes have been shown to follow SE, such as reorganization of excitatory axons (Sutula et al., 1989), altered function of excitatory neurotransmitter receptors (Turner and Wheal, 1991; Lothman et al., 1995; Chen et al., 1999), or changes in GABA_A receptor-mediated inhibition (Mangan et al., 1995; Gibbs et al., 1997; Brooks-Kayal et al., 1998; Cossart et al., 2001). Many of these synaptic changes have been suggested to contribute to the development of temporal lobe epilepsy (TLE) that is frequently the outcome of a single or multiple episodes of SE.

Much less is known about SE-induced changes in intrinsic neuronal properties. However, a recent study in the pilocarpine model, in which an episode of SE induced by the convulsant pilocarpine progresses to a chronic epileptic condition resembling human TLE (Turski et al., 1983), suggests that such alterations may be highly significant. In this model, Sanabria et al. (2001) found a marked upregulation of intrinsic neuronal bursting associated with the development of TLE. Although almost all pyramidal neurons in the hippocampal CA1 area are regular firing cells in normal conditions (Jensen et al., 1994), ~50% of CA1 pyramidal cells in hippocampal tissue removed from rats that experienced SE were found to be intrinsically burst-firing cells. Moreover, the upregulation of intrinsic bursting seemed to result from the de novo appearance of Ca²⁺-dependent bursting that is not ordinarily seen in this class of principal hippocampal neurons (Azouz et al., 1996). It was also found that a subset of the newly formed bursters, namely, the spontaneously bursting pyramidal cells, acted as pacemakers of spontaneous interictal-like epileptiform bursts, recruiting the entire CA1 population of pyramidal cells, nonbursters and bursters alike, into synchronized discharge (Sanabria et al., 2001).

Because the switch in neuronal firing mode after SE may be important for the development and expression of TLE, and because it may represent a novel mechanism of activity-induced neuronal plasticity, we have used a combination of electrophysiological and pharmacological techniques to characterize in detail the ionic mechanisms underlying the increased intrinsic bursting. Here we report that the dramatic change in firing mode of CA1 neurons after SE is most probably caused by the increased density of a Ni²⁺-sensitive T-type Ca²⁺ current. Our findings demonstrate that epilepsy-related changes in intrinsic neuronal properties may result from activity-dependent differential regulation of specific ion channel subtypes and suggest that subunit-selective T-type channel antagonists may be promising future targets for rational anti-epileptic drug design.

	MATERIALS AND METHODS

TOP ABSTRACT INTRODUCTION MATERIALS AND METHODS RESULTS DISCUSSION REFERENCES

Induction of SE. Experimental protocols were approved by the local animal care and use committees. Male Sabra or Wistar rats (150-200 gm) were injected with a single high dose of the muscarinic agonist pilocarpine (300-380 mg/kg, i.p.), which induced SE in most (~80%) animals. Peripheral muscarinic effects were reduced by previous administration of methyl-scopolamine (1 mg/kg, s.c.; 30 min before injection of pilocarpine). Diazepam (0.1 mg/kg, s.c.) was administered to all animals 2 hr after the pilocarpine injection. It terminated the convulsions in the responsive rats and sedated all animals. Experiments were performed on hippocampal slices from rats that experienced SE after pilocarpine injection (SE-experienced rats) and from those that did not (sham-control rats). A third group of untreated, age-matched rats served as an additional control (naive-control rats). Previous work has found no differences in electrophysiological properties between sham- and naive-control rats (Sanabria et al., 2001).

Preparation of hippocampal slices and dissociated neurons. Animals were decapitated under ether anesthesia 6-40 d after pilocarpine treatment, and transverse hippocampal slices (250 or 400 µm) were prepared with a vibrating microslicer (Campden Instruments or Leica) and transferred to a storage chamber perfused with oxygenated (95% CO₂-5% O₂) artificial CSF (ACSF) containing (in mM): NaCl 125, KCl 3, NaH₂PO₄ 1.25, MgCl₂ 1, CaCl₂ 2, NaHCO₃ 25, and glucose 20, pH 7.4, osmolarity 305 mOsm, where they were maintained at room temperature. For intracellular recordings, 400-µm-thick hippocampal slices were placed in an interface chamber (33.5°C) and perfused with oxygenated ACSF containing (in mM): NaCl 124, KCl 3.5, NaH₂PO₄ 1.25, MgSO₄ 2, CaCl₂ 2, NaHCO₃ 26, and D-glucose 10. In experiments in which Ni²⁺ was used, NaH₂PO₄ was omitted. Ca²⁺ channel blockers, or the glutamate receptor antagonists 6-cyano-7-nitro-quinoxaline-2,3-dione (CNQX) and 2-amino-5-phosphono-valeric acid (APV), were added to the ACSF as indicated. For patch-clamp recordings in the slice preparation, 250 µM hippocampal slices were placed in a submerged recording chamber (21-24°C) and perfused continuously (2.5 ml/min) with oxygenated ACSF containing (in mM): NaCl 125, KCl 2.5, NaHCO₃ 26.7, CaCl₂ 2.5, MgCl₂ 1, HEPES 13, glucose 12.5, pH 7.3, osmolarity 300 mOsm. Pyramidal cells in the CA1 field were visualized at 400× magnification with Dodt-Gradient-Contrast optics (Luigs and Neumann) using a Zeiss Axioskop microscope and an infra-red video camera (Hamamatsu, Shizuoka, Japan).

Dissociated hippocampal neurons were prepared from 400-µm-thick slices primarily as described previously (Beck et al., 1999). After an equilibration period (>60 min), enzymatic digestion was performed for 10 min at 37°C and 5 min at room temperature in 5 ml of incubation medium containing (in mM): sodium methanesulfonate 145, KCl 3, CaCl₂ 0.5, MgCl₂ 1, HEPES 10, glucose 15, and 2 mg/ml pronase (protease type XIV; Sigma, St. Louis, MO) (pH 7.4, osmolarity 310 mOsm, 100% O₂). After washing with enzyme-free incubation medium, the CA1 region was dissected and triturated with fire-polished glass pipettes. The cell suspension was placed in a Petri dish and superfused with modified ACSF containing (in mM): sodium methanesulfonate 125, tetraethylammonium chloride (TEA) 20, 4-aminopyridine 4, BaCl₂ 5, MgCl₂ 1, KCl 3, glucose 10, HEPES 10, tetrodotoxin (TTX) 0.5 µM, pH 7.4, osmolarity 315 mOsm. Cells were visualized on a inverted microscope (Zeiss Axiovert).

Sharp microelectrode recordings in slices. Intracellular recordings were obtained using sharp glass microelectrodes containing 1 M K⁺-acetate (70-90 M). An active bridge circuit in the amplifier (Axoclamp 2B, Axon Instruments) allowed simultaneous injection of current and measurement of membrane potential. The signals were filtered on-line at 5 kHz, digitized at a sampling rate of 10 kHz, and stored on hard disk (TL-1 DMA and pClamp, Axon Instruments). In some experiments, bipolar platinum (50 µm) electrodes connected to a stimulator by an isolation unit were used for focal stimulation of afferent fibers in stratum radiatum near the CA2/CA3 border (orthodromic stimulation).

Patch-clamp recordings in slices and dissociated neurons. Recording patch pipettes (2-4 M) were pulled from borosilicate glass on a vertical puller (List-Medical or Narishige, Tokyo, Japan). Pipettes were coated with Sylgard resin for recordings in the slice preparation (Dow Corning Chemical) and filled with an intracellular solution containing (in mM): Cs-methanesulfonate 100, EGTA 5, HEPES 10, TEA 20, MgCl₂ 2, CaCl₂ 0.1, pH 7.35. For recordings from dissociated CA1 neurons, pipettes were filled with (in mM): Cs-methanesulfonate 87.5, TEA 20, CaCl₂ 0.5, MgCl₂ 5, BAPTA 5, HEPES 10, glucose 10, Na⁺2-ATP 10, and GTP 0.5, pH 7.2 (NaOH), osmolarity adjusted to 300 mOsm with sucrose. Tight-seal whole-cell recordings were obtained using a patch-clamp amplifier (Axopatch 200A, Axon Instruments, or EPC9, HEKA Instruments). The signals were collected on-line as described above. Series resistance compensation was used to improve the voltage-clamp control (60-85%) so that the maximal residual voltage error did not exceed 5 mV. A liquid junction potential of ~10 mV was measured between the intracellular and extracellular solutions and corrected on-line.

Chemicals and drugs. In slice experiments the drugs were applied via the perfusing ACSF. Application of drugs to dissociated neurons was performed via a pipette placed at a distance of 30-50 µm from the cell body. All drugs were obtained from Sigma, except the Ca²⁺ channel toxins (Bachem or Alomone Labs) and CNQX (Tocris Neuroamin). Stock solutions of the toxins (0.2-1 mM) were prepared in deoxygenated solution containing 0.1% BSA, 100 mM NaCl, 10 mM Trizma, 1 mM EDTA, pH 7.5. In experiments using the toxins, all solutions contained 0.1 mg/ml cytochrome c to prevent unspecific peptide binding to tubing. Stock solutions (10 mM) of nifedipine and nicardipine were prepared in DMSO.

Analysis. A measure for the size of the spike afterdepolarization was provided by the area delimited by the ADP waveform and resting membrane potential. The concentration-dependent reduction of Ca²⁺ current amplitude was fit with a modified Hill function of the form: E = E_max * cⁿ/(cⁿ + IC₅₀ⁿ), where E is the fraction of current blocked, E_max corresponds to the maximal block, c is the concentration of antagonist, n is the Hill coefficient, and the IC₅₀ is the concentration at which half-maximal blocking effects were observed.

The decay of tail currents after mock action potentials was fit with a biexponential equation of the form: I(t) = A₁ * (1  exp(t/_f)) + A₂ * (1  exp(t/_s)), where I(t) is the current amplitude at the time point t after onset of the voltage command, _f and _s are the fast and slow decay time constants, respectively, and A is the amplitude contribution of the different time constants. Data were fit using a Levenberg-Marquard nonlinear curve-fitting procedure.

Significant differences between groups were tested with a two-tailed Student's t test with the significance level set to p < 0.05.

	RESULTS

TOP ABSTRACT INTRODUCTION MATERIALS AND METHODS RESULTS DISCUSSION REFERENCES

Altered intrinsic bursting after pilocarpine-induced SE

First, we have replicated the recent findings of Sanabria et al. (2001), demonstrating enhanced bursting behavior in SE-experienced rats compared with naive-control and sham-control animals, in a new set of experiments. Sharp microelectrodes were used to impale CA1 pyramidal cells and to stimulate them with threshold-straddling, long (200 msec) and brief (4 msec) depolarizing current pulses (Azouz et al., 1996). In both the naive-control (n = 15 cells; data not shown) and sham-control (n = 42 cells) (Fig. 1A) groups, all except one neuron fired a series of independent spikes in response to the long pulse and a single spike in response to the brief pulse (Fig. 1Aa,B). The remaining neuron in each group burst-fired in response to the long pulse. In marked contrast, more than half of the CA1 neurons in the SE-experienced group (54%; n = 97) generated a burst of action potentials as a minimal response to threshold-straddling long current injections and in many cases burst-fired also in response to brief stimulation (Fig. 1Ab,B). As expected (Sanabria et al., 2001), the burst responses were unaffected by blocking synaptic transmission with CNQX (15 µM), APV (50 µM), and bicuculline methiodide (10 µM; n = 26). Thus, as described previously, pilocarpine-induced SE triggers a long-lasting switch in firing mode from a nonbursting to a bursting behavior in a large fraction of CA1 pyramidal cells.

View larger version (14K): [in this window] [in a new window]   Figure 1.   Upregulation of intrinsic burst-firing in CA1 pyramidal cells from SE-experienced versus control animals. A, Representative responses of CA1 pyramidal cells from sham-control (a) and SE-experienced animals (b) 30 d after pilocarpine treatment. In each panel, the responses of CA1 pyramidal cells to long (leftmost traces) and brief (rightmost traces) depolarizing current pulses (injected through the recording microelectrode) are shown. Top and bottom traces depict the neuronal response and the current stimulus, respectively. B, Most of the CA1 pyramidal cells in the sham-control (n = 42) as well as in the naive-control group (n = 15) were regular firing cells, with only a small fraction displaying burst discharges to threshold stimulation (white bars). In contrast, CA1 pyramidal cells in the SE-experienced group showed a high incidence of intrinsic bursting (54%, n = 97), with bursting neurons displaying all-or-none bursts of three to four clustered spikes in response to either brief or long current injection (Ab).

Critical role of Ni²⁺-sensitive Ca²⁺ channels in SE-induced intrinsic bursting

Previous work has suggested that Ca²⁺ currents play a critical role in the SE-induced intrinsic bursting of CA1 pyramidal cells (Sanabria et al., 2001). In normal tissue, CA1 pyramidal cells express multiple types of voltage-gated Ca²⁺ channels, namely, L-, N-, P-/Q-, R-, and T-types (Yaari et al., 1987; Takahashi et al., 1989; Fisher et al., 1990; Thompson and Schwindt, 1991; Christie et al., 1995). To identify the Ca²⁺ channel types that mediate intrinsic bursting induced by SE, we have compared the effects of selective organic Ca²⁺ channel blockers: namely, nicardipine (10 µM; n = 6) or nifedipine (30 µM; n = 5) to block L-type, -conotoxin GVIA (1 µM; n = 7) or neomycin (0.5 mM; n = 6) to block N-type, -conotoxin MVIIC (5 µM; n = 5) to block N-/P-/Q-type, and -agatoxin TK (300 nM; n = 3) to block P-type Ca²⁺ channels. Additionally, the divalent cation Ni²⁺ was applied at low concentrations (50-100 µM; n = 32) that predominantly block T-/R-type Ca²⁺ channels (Soong et al., 1993; Williams et al., 1994; Lee et al., 1999b). The blockers were added to the ACSF perfusing the slices from SE-experienced animals for at least 45 min. The dihydropyridines (Fig. 2A, compare a, b) did not affect bursting in any of the neurons tested, and neither did neomycin (data not shown) or the toxin blockers of Ca²⁺ channels (Fig. 2B-D, compare a, b).

View larger version (22K): [in this window] [in a new window]   Figure 2.   Critical role of Ni2+-sensitive Ca2+ channels in intrinsic burst firing in SE-experienced animals. Recordings were performed on intrinsically bursting CA1 neurons from SE-experienced rats (Aa, Ba, Ca, and Da). A-D, No change in intrinsic bursting behavior could be observed after 40 min of perfusion with 10 µM nicardipine (Ab) or 1 µM -conotoxin GVIA (Bb; 30 min). Likewise, application of 5 µM -conotoxin MVIIC (Cb; 40-80 min) or 300 nM -agatoxin TK (Db; 40-60 min) did not affect intrinsic burst generation. In all cases, additional perfusion of 50 µM Ni2+ blocked bursting entirely (Ac, Bc, Cc, and Dc).

To test whether intrinsic bursting is generated synergistically by several types of Ca²⁺ channels, we have added the organic Ca²⁺ channel blockers sequentially to the ACSF (without washing them out) while recording from a single neuron. In these experiments (n = 5), intrinsic bursting was unaffected in all cases (Fig. 3Aa₁-d₁). In contrast, when 50 or 100 µM Ni²⁺ was added to the ACSF containing one or more of the organic Ca²⁺ channel blockers, intrinsic bursting was entirely suppressed in 26 of 32 (81%) neurons (Figs. 2Ac-Dc, 3Ae₁). To confirm that the organic Ca²⁺ channel blockers are pharmacologically active when applied to the slice, we monitored their effects on the orthodromically evoked EPSPs. In all experiments, -conotoxin MVIIC, -conotoxin GVIA, -agatoxin TK, and nicardipine produced a partial reduction of the EPSPs within 30 min (Fig. 3Aa_2-d₂), presumably consequent to blocking a subset of presynaptic voltage-gated Ca²⁺ channels (Wu and Saggau, 1994; Qian and Noebels, 2001).

View larger version (13K): [in this window] [in a new window]   Figure 3.   Combined application of organic Ca2+ channel antagonists fails to block bursting. A, Ca2+ channel blockers were sequentially added to the ACSF, and the efficacy of Ca2+ channel blockade was assessed by the progressive block of the EPSP evoked by orthodromic stimulation of the Schaffer collaterals (Aa2-Ae2). Combined application of organic Ca2+ antagonists did not block bursting (Aa1-Ad1) but additional application of 50 µM Ni2+ did (Ae1). Blockers were applied for at least 30 min (-conotoxin GVIA 1 µM, 62 min; -agatoxin TK 300 nM, 40 min; nicardipine 10 µM, 30 min; Ni2+ 50 µM, 50 min).

We also examined the consequences of blocking only T-/R-type Ca²⁺ channels with low concentrations of Ni²⁺. Addition of 10 µM Ni²⁺ to the ACSF had no effect on intrinsic bursting (n = 4), but 30 µM Ni²⁺ shortened the bursts in two of four neurons. Addition of 100 µM Ni²⁺ to the ACSF reversibly suppressed intrinsic bursts in 35 of 42 (83%) bursters examined (Fig. 4Aa₁-c₁). Raising the concentration of Ni²⁺ further (up to 1 mM) did not block intrinsic bursts that were insensitive to 100 µM Ni²⁺ (n = 5; data not shown), indicating that Ni²⁺-insensitive bursting is not mediated by any type of voltage-gated Ca²⁺ channel. Rather, it may involve activation of persistent Na⁺ channels (Azouz et al., 1996; Su et al., 2001), but this mechanism was not investigated further in this study.

View larger version (25K): [in this window] [in a new window]   Figure 4.   Low concentrations of Ni2+ suppress burst firing by reducing the spike ADP. A, Intrinsically bursting CA1 pyramidal neuron from an SE-experienced animal in normal ACSF (a1), after block of the burst discharge by perfusion of 50 µM Ni2+ (b1), and after washout (c1). The slow depolarization underlying the burst was unmasked by delivering a brief (4 msec) hyperpolarizing current pulse immediately after the first spike (a2-c2). The time course of the ADP was similar in a1 and a2 (for comparison at larger magnification, see d). Adding 50 µM Ni2+ to the ACSF reversibly suppressed the ADP (b2, c2; for comparison at larger magnification, see e). B, Regular firing CA1 pyramidal cell in a sham-control animal before (a) and after (b) application of 100 µM Ni2+. The ADP was not affected by Ni2+ (for comparison at larger magnification, see c).

Low concentrations of Ni²⁺ suppress intrinsic bursting by reducing the spike afterdepolarization

In CA1 pyramidal cells, the fast spike activates a slow somatodendritic inward current that generates a slow spike ADP in the soma. Although in regular firing cells the ADP is subthreshold, in bursters it redepolarizes the neuron sufficiently to generate additional spikes (Azouz et al., 1996). We tested in four bursters whether low Ni²⁺ concentrations suppress the spike ADP underlying the burst discharge. This slow potential was unmasked by delivering a brief (4 msec) hyperpolarizing current pulse immediately after the first spike. The intensity of this pulse was adjusted to the minimum required to inhibit further discharge (Wong and Prince, 1981; Jensen et al., 1996). This procedure disclosed a large ADP with a duration similar to that of the depolarizing burst envelope (Fig. 4Aa₁,a₂; overlaid and enlarged in d). Adding 50 µM Ni²⁺ to the ACSF suppressed the burst discharge (Fig. 4Aa₁,b₁) and concurrently attenuated the size of the ADP in these cells (Fig. 4Aa₂,b₂; overlaid and enlarged in e). We also examined the effect of low Ni²⁺ concentrations on the spike ADP in six regular firing CA1 pyramidal cells in sham-control hippocampal slices. The spike ADPs in these neurons were significantly smaller than in neurons from SE-experienced animals (108.0 ± 5.1 vs 250.8 ± 7.1 mV · msec, respectively) and were insensitive to 100 µM Ni²⁺ (Fig. 4Ba,b; overlaid and enlarged in c). The Ni²⁺-insensitive ADP components most likely are generated by persistent Na⁺ current (Azouz et al., 1996; Su et al., 2001).

Depolarization from resting membrane potential abolishes intrinsic bursting

These data so far have suggested that in CA1 pyramidal cells from SE-experienced animals, Ni²⁺-sensitive, T-/R-type Ca²⁺ current furnishes the main depolarizing drive for the spike ADP leading to burst generation. Both T- and R-type Ca²⁺ channels are steeply voltage-dependent and manifest inactivation after depolarization from the resting membrane potential (Randall and Tsien, 1997; Kozlov et al., 1999). To further explore their role in bursting, we tested how depolarization with constant current injection affects this activity. In five of seven neurons examined, the burst responses were suppressed by depolarizing the neurons 3-5 mV from their resting membrane potential (Fig. 5, compare Aa, Ba). Depolarizing these neurons by >5 mV suppressed the burst responses in all cases and induced the appearance of spontaneous single spike firing. Although there may be other explanations, these results are consistent with the notion that bursting is generated by T-/R-type Ca²⁺ currents. Further supporting this notion was the finding that although Ni²⁺ suppressed bursting at resting membrane potential presumably by reducing the spike ADP (Fig. 5Aa,b; overlaid and enlarged in Ac), it had no effect on the spike ADP at the slightly more depolarized potentials (Fig. 5Ba,b; overlaid and enlarged in Bc).

View larger version (20K): [in this window] [in a new window]   Figure 5.   Modest depolarization from resting potential suppresses burst discharges. A, Pyramidal neuron from an SE-experienced animal showing Ni2+-sensitive bursting (compare a, b; for comparison at larger magnification, see c). B, Depolarization of the neuron from a resting potential of 61 mV to a potential of 58 mV (compare Aa, Ba) converts the burst discharge into a single spike. Under these conditions, Ni2+ did not affect the time course of the spike ADP (compare Ba, Bb; for comparison at larger magnification, see c).

Increase in T-type Ca²⁺ current density in SE-experienced animals

The de novo appearance of Ni²⁺-sensitive intrinsic bursting in CA1 pyramidal cells described above might be caused by a genuine increase in the density of functional T-/R-type Ca²⁺ channels, a more effective recruitment of existing channels by the first somatodendritic spike, or both. We have therefore directly measured the densities of T- and R-type Ca²⁺ currents in CA1 pyramidal cells in naive-control and SE-experienced rats using the whole-cell patch-clamp technique.

We first compared the densities of these currents between the two experimental groups in visually identified CA1 pyramidal cells in hippocampal slices. Voltage steps from 90 to 60 and 50 mV evoked transient Ca²⁺ currents (Fig. 6Aa) (example shown for 60 mV voltage steps). The densities of these currents were significantly larger (2.2-fold and 1.9-fold increase for command pulses to 60 and 50 mV, respectively; p < 0.01) in SE-experienced animals (n = 10 cells; 6-12 d after pilocarpine-induced SE) compared with the naive-control animals (n = 12 cells) (Fig. 6Ac).

View larger version (20K): [in this window] [in a new window]   Figure 6.   Increased density of T-type Ca2+ currents in SE-experienced animals. A, Recordings of T-type Ca2+ current in a CA1 pyramidal cell in the slice preparation using voltage steps from 90 to 60 or 50 mV (a) or in a dissociated CA1 neuron perfused with ACSF containing 2 µM -conotoxin GVIA, 3 µM -conotoxin MVIIC, 200 nM -agatoxin GIVA, and 10 µM nifedipine to block most of the high-voltage-activated Ca2+ channel types (b; see also Fig. 8Ab). In this preparation, Ca2+ currents were evoked with voltage steps to 50 mV from a holding potential of 80 mV after a conditioning prepulse to 100 mV (5 sec). Average T-type amplitudes measured in SE-experienced versus naive-control animals in either CA1 neurons in slices (n = 10 and 12, respectively) or dissociated CA1 neurons (n = 14 and 15, respectively) are depicted in c. The current amplitudes were normalized to the cell capacitance in all cases. The current density showed a significant increase in SE-experienced animals (black bars) compared with naive-control animals (white bars) for recordings from both dissociated and intact CA1 neurons (*p < 0.05). B, Ni2+ sensitivity of the T-type current in dissociated CA1 neurons. The T-type current was markedly and reversibly reduced by micromolar concentrations of Ni2+, as shown in an exemplary recording from an SE-experienced animal (a). Concentration-dependence of the T-type Ca2+ current block by Ni2+ in both SE-experienced () and naive-control groups () (SE-experienced group: n = 3, 6, 6, and 3 cells; naïve-control group: n = 4, 2, 7, and 5 cells for 10, 30, 100, and 300 µM Ni2+; b). Data were fit by a Hill equation using a Levenberg-Marquard nonlinear curve-fitting procedure. The fitting curve is shown superimposed on the data points.

Similar experiments were performed in acutely dissociated CA1 pyramidal cells using depolarizing voltage steps to 50 mV preceded by a 5 sec prepulse to 100 mV (Fig. 6Ab). In these experiments we also superfused the neurons with ACSF containing organic Ca²⁺ channel blockers (2 µM -conotoxin GVIA, 3 µM -conotoxin MVIIC, 200 nM -agatoxin GIVA, and 10 µM nifedipine) to avoid even a small contribution of N-, P/Q-, or L-type Ca²⁺ channels (Avery and Johnston, 1996). As found in the slice preparation, the densities of T-type Ca²⁺ currents in dissociated CA1 pyramidal cells were significantly larger (3.3-fold increase; p = 0.0001) in SE-experienced (n = 14 cells; 30-40 d after SE) compared with naive-control animals (n = 15 cells) (Fig. 6Ac).

Ni²⁺ sensitivity of T-Type Ca²⁺ current in SE-experienced animals

Recent studies of voltage-gated Ca²⁺ channels have identified three pore-forming ₁ subunits, namely, _1G, _1H, and _1I, that give rise to T-type Ca²⁺ channels (Cribbs et al., 1998; Perez-Reyes et al., 1998; Lee et al., 1999a). All three subunits are expressed in hippocampal CA1 pyramidal cells (Talley et al., 1999). They differ, however, in their sensitivity to blockage by Ni²⁺, with _1H being an order of magnitude more sensitive to Ni²⁺ than _1G and _1I (Lee et al., 1999b). We have therefore examined the Ni²⁺ sensitivity of the T-type Ca²⁺ current in these neurons in SE-experienced as well as in the naive-control animals. In both groups, 100 µM Ni²⁺ almost completely and reversibly blocked the T-type Ca²⁺ current (Fig. 6Ba). Dose-response curves for Ni²⁺ (10-300 µM) (Fig. 6Bb) yielded similar IC₅₀ values for SE-experienced (24.6 ± 2.6 µM; maximal block 84.5 ± 4.1%) and naive-control animals (27.9 ± 1.6 µM; maximal block 79.6 ± 2.0%).

T-type Ca²⁺ currents invariably show characteristically slow deactivation rates that distinguish them from the much more rapidly deactivating R-type channels (Randall and Tsien, 1997; Nakashima et al., 1998; Kozlov et al., 1999). Therefore, tail currents after brief depolarizing steps that activate both T- and R-type Ca²⁺ currents may be used to analyze these two current components separately. As illustrated in Figure 7Aa, activation of pharmacologically isolated T-/R-type Ca²⁺ currents by mock action potentials as voltage commands was followed by biphasic tail currents in both experimental groups of neurons. These currents were best fitted by a biexponential curve (Fig. 7Ab). The fast (_f) and slow (_s) decay time constants of these tail currents were, respectively, 478 ± 275 µsec and 4.1 ± 2.5 msec in naive-control animals (n = 7 cells), and 712 ± 122 µsec and 4.7 ± 1.6 msec in SE-experienced animals (n = 5 cells). The rapidly deactivating component most probably corresponds to an R-type current, whereas the slowly deactivating component is caused by T-type Ca²⁺ currents (Kozlov et al., 1999). Indeed, the amplitude of the slowly deactivating component of the tail current derived from biexponential fitting was tightly correlated with the amplitude of the T-type Ca²⁺ current measured with rectangular voltage steps (correlation coefficient 0.88; p = 0.0005; n = 12 cells). The amplitude of the slow (presumably T-type) tail Ca²⁺ current component was considerably larger in the SE-experienced group than in the control group (3.9-fold increase; p = 0.005), whereas that of the rapid (presumably R-type) component was not different (Fig. 7B). These results support our conclusion of a selective upregulation of T-type Ca²⁺ current in CA1 pyramidal cells in SE-experienced animals.

View larger version (21K): [in this window] [in a new window]   Figure 7.   Increased T-type Ca2+ currents after SE are associated with an increase in slowly deactivating Ca2+ tail currents after mock action potentials. A, Application of mock action potentials (rising phase 1 msec; decaying phase 2 msec; peak +30 mV) as a voltage command in dissociated CA1 pyramidal neurons from naive-control animals (a1) and SE-experienced animals (a2). Current traces were derived by subtraction of traces obtained in the presence of organic Ca2+ blockers and 300 µM Ni2+ from traces obtained only in the presence of organic Ca2+ channel blockers and thus reflect Ca2+ influx through T-/R-type channels. The decay of the inward tail current immediately after termination of the mock action potential was fit by a biexponential equation superimposed on the data points (b). B, Amplitudes of the fast and slowly decaying component of the tail currents normalized to the cell capacitance. A significant increase was observed only for the slower decaying component (*p < 0.005).

Changes in densities of high voltage-activated Ca²⁺ currents in SE-experienced animals

In the slice preparation, voltage steps to potentials above 40 mV evoked large Ca²⁺ currents that escaped voltage-clamp control in neurons from both experimental groups. Therefore, changes in the densities of high voltage-activated Ca²⁺ currents were investigated only in acutely dissociated CA1 pyramidal cells, in which these currents could be adequately voltage clamped (Beck et al., 1999). Stepping the membrane voltage from 100 to 0 mV evoked large Ca²⁺ currents (69.5 ± 4.0 pA/pF in naïve control animals; 69.0 ± 5.7 pA/pF in SE-experienced animals), which were reduced to approximately one-third by perfusing the neurons with ACSF containing the organic Ca²⁺ channel blockers (Fig. 8Aa,b). The residual current evoked with test pulses to 0 mV comprises mostly R-type Ca²⁺ currents, with a small contribution of T-type currents (Thompson and Schwindt, 1991). Despite the increase in T-type current amplitude, the density of the compound T-/R-type current was not different between SE-experienced (n = 21) and naive-control neurons (n = 20) (Fig. 8Ac), indicating that the R-type current is either unaltered or slightly reduced. This conclusion is supported also by the lack of change in amplitude of the rapidly decaying tail Ca²⁺ current component after mock action potentials (Fig. 7B).

View larger version (24K): [in this window] [in a new window]   Figure 8.   Functional analysis of high-threshold current components. A, Recordings were obtained in a dissociated CA1 pyramidal neuron from a naive-control animal. Ca2+ currents were evoked with the voltage paradigm shown in the inset. To isolate the T-/R-type Ca2+ current, the organic blockers -conotoxin GVIA (2 µM), -conotoxin MVIIC (3 µM), -agatoxin GIVA (200 nM), and nifedipine (10 µM) were co-applied, unmasking a rapidly inactivating residual component (a). The current traces in a were recorded at the time points indicated by the lowercase letters in b. Pharmacologically isolated T-/R-type Ca2+ currents were compared in dissociated CA1 pyramidal neurons from SE-experienced (n = 21 cells) and naive-control animals (n = 20 cells) (c). Current densities were obtained by normalizing current amplitudes to cell capacitance. B, In another dissociated neuron from a naive-control animal, the organic Ca2+ channel blockers -conotoxin GVIA (2 µM), -agatoxin IVa (200 nM), and nifedipine (10 µM) were added sequentially (a; duration of application is indicated by horizontal bars, b). This allowed assessment of the individual contributions of N-, P/Q-, and L-type Ca2+ current components to the whole-cell current (indicated at right margin of b). The current traces in a were recorded at the time points indicated by the lowercase letters in b. High-voltage-activated Ca2+ current densities in naïve control (n = 9-10) versus SE-experienced rats (n = 10) are shown in c. The N-type current density was significantly reduced (*p < 0.05), whereas the density of P/Q- and L-type currents was unaltered.

We also compared the densities of Ni²⁺-insensitive, high-threshold Ca²⁺ currents in acutely dissociated CA1 pyramidal cells from SE-experienced versus naive-control animals. The amplitudes of N-, P/Q-, and L-type Ca²⁺ currents were determined by sequentially applying the selective antagonists 2 µM -conotoxin GVIA (n = 10 for both groups), 200 nM -agatoxin IVa (n = 10 for both groups), and 10 µM nifedipine (naive-control, n = 9 cells; SE-experienced, n = 10 cells), respectively (Fig. 8Ba,b). The effects of -conotoxin GVIA and -agatoxin IVa were primarily irreversible (Fig. 8Bb). The N-type Ca²⁺ current density was significantly reduced in the SE-experienced compared with the naive-control group, whereas the densities of P/Q- and L-type currents were not significantly altered (Fig. 8Bc). Thus, of all the different types of Ca²⁺ currents expressed in CA1 pyramidal neurons, only T-type Ca²⁺ channel density is upregulated in SE-experienced animals.

Impact of altered firing mode on neuronal responses to synaptic excitation

The conversion of CA1 pyramidal cells from regular firing to burst firing after pilocarpine-induced SE would be expected to amplify their spike output in response to excitatory synaptic inputs. To examine this notion, we compared the synaptic activation of regular firing neurons in sham-control animals (Fig. 9Aa) (n = 8 cells) with that of bursting neurons in SE-experienced animals (Fig. 9Ba) (n = 4 cells). Single-shock stimuli were applied to afferent fibers in stratum radiatum, and their intensity was adjusted to evoke threshold-straddling EPSPs (Fig. 9Ab,Bb). As expected, the minimal response in sham-control animals was a single spike (Fig. 9Ab). In contrast, the minimal response in SE-experienced animals was a spike burst similar in pattern to that evoked by direct current injection (Fig. 9Bb). To confirm that in the latter group the threshold EPSPs recruit the intrinsic burst mechanism rather than produce multiple spiking by virtue of their longer duration (Fig. 9, compare top panels in Ab, Bb), we exposed them to Ni²⁺. Because a small blocking effect of Ni²⁺ was observed on EPSPs, the stimulus strength was readjusted to yield threshold EPSPs. Adding 100 µM Ni²⁺ to the ACSF suppressed the intrinsic burst response (Fig. 9Bc) and reduced the burst responses to threshold EPSPs to single spikes (Fig. 9Bd) without affecting the duration of these EPSPs (Fig. 9Ba,c, top traces). These data clearly demonstrate that SE, by modifying intrinsic neuronal properties of CA1 pyramidal cells, markedly and persistently amplifies the neuronal output to a given synaptic input.

View larger version (22K): [in this window] [in a new window]   Figure 9.   Impact of intrinsic plasticity on neuronal responses to synaptic excitation. These experiments were performed in the absence of blockers of synaptic transmission in the control ACSF. A, Recordings from a regular firing CA1 pyramidal cell from a sham-control animal. Firing behavior was determined using long depolarizing current injections through the recording microelectrode (a). Single-shock stimuli were applied to afferent fibers in stratum radiatum and adjusted to evoke threshold-straddling EPSPs (b; different trials with identical stimulation intensity are shown). B, A similar experiment in a bursting neuron (a) from an SE-experienced animal (n = 4 cells). All suprathreshold EPSPs elicited a burst discharge (b; three different trials with identical stimulation intensity; 1.4 V). Application of 100 µM Ni2+ blocked the intrinsic bursts induced by depolarizing current pulses (compare a, c). It also slightly reduced the amplitude of the EPSPs without affecting their duration (data not shown). To elicit threshold EPSPs in the presence of 100 µM Ni2+, stimulation intensity was increased to 1.5 V (d, top trace). Under these conditions, the EPSP-evoked firing responses were converted to single spikes (d; middle and bottom traces).

	DISCUSSION

TOP ABSTRACT INTRODUCTION MATERIALS AND METHODS RESULTS DISCUSSION REFERENCES

In this study we demonstrate that the intrinsic discharge behavior of hippocampal CA1 neurons is dramatically modified after pilocarpine-induced SE, in congruence with another recent study (Sanabria et al., 2001). This form of plasticity consists of a transition from regular firing to a burst-firing mode, in which the minimal response of >50% of the neurons to threshold depolarization is a burst of several spikes. We also show that this abnormal burst activity is resistant to blockers of L-, N-, and P/Q-types of voltage-sensitive Ca²⁺ channels but is readily suppressed by low concentrations of Ni²⁺ that block R- and T-types. Furthermore, we show that the appearance of Ni²⁺-sensitive intrinsic bursting is associated with a marked increase in the density of T-type, but not R-type, Ca²⁺ channels. Cumulatively, these data suggest that an increase in T-type Ca²⁺ current density plays a critical role in the intrinsic neuronal plasticity that is triggered by a single episode of SE.

Role of T-type Ca²⁺ current in intrinsic neuronal plasticity

It was shown previously that SE-induced intrinsic bursting in pilocarpine-treated animals is suppressed by removal of Ca²⁺ from, or the addition of 1 mM Ni²⁺ to, the ACSF, but not by the intracellular application of a Ca²⁺ chelator, suggesting that this activity is driven directly by a Ca²⁺ current (Sanabria et al., 2001). Our further pharmacological experiments show that none of the organic Ca²⁺ channel blockers that affect L-, N-, and P-/Q-type Ca²⁺ channels, applied individually or in combination, blocked intrinsic bursting in this model. In contrast, both intrinsic bursting and its underlying spike ADP were suppressed by low concentrations of Ni²⁺ (30-100 µM), which block both T- and R-type Ca²⁺ channels in CA1 pyramidal cells. In addition, moderate depolarization of the neuron from its resting membrane potential, which would augment the steady-state inactivation of both T- and R-type Ca²⁺ channels (Schneider et al., 1994; Kozlov et al., 1999), abolished intrinsic bursting. These results by themselves are consistent with a role of either T- or R-type Ca²⁺ channels in intrinsic burst generation.

Two major lines of evidence, however, argue for a critical role of T-type Ca²⁺ channels in mediating this activity. First, the density of T-type Ca²⁺ current was considerably (1.9- to 3.3-fold) increased in CA1 pyramidal cells after SE, whereas the density of all other types of Ca²⁺ current (including the R-type) was either unaltered or decreased. Second, T-type Ca²⁺ currents display biophysical characteristics that make them particularly suitable to mediate burst discharges (Huguenard, 1996). Thus, T-type, but not R-type, Ca²⁺ channels display a slow rate of deactivation (time constants in the order of several milliseconds) at potentials close to the neuronal resting potential (Randall and Tsien, 1997; Kozlov et al., 1999). As a consequence of this feature, action potentials induce a slow tail Ca²⁺ current mediated by T-type Ca²⁺ currents. We have found that the increase in T-type Ca²⁺ current amplitude after SE is associated with a marked and selective increase of the slowly deactivating tail current component after mock action potentials. Clearly, an increase in slow inward currents after action potentials could initiate a regenerative depolarization that would boost the ADP beyond spike threshold and elicit additional discharge. Additionally, the low threshold for activation and enhanced deinactivation during hyperpolarization of T-type Ca²⁺ channels would allow them to furnish the initial depolarizing drive for spontaneous burst discharges (Huguenard, 1996).

In normal CA1 pyramidal cells, intrinsic bursting mediated by Ca²⁺ currents has been demonstrated only after blocking outward K⁺ currents by millimolar concentrations of 4-aminopyridine (Magee and Carruth, 1999). However, in that condition, bursting was generated by both Ni²⁺-sensitive and Ni²⁺-insensitive Ca²⁺ currents (Magee and Carruth, 1999), reflecting the complement of voltage-gated Ca²⁺ channels normally expressed in these neurons. It is improbable, therefore, that a persistent reduction in outward K⁺ currents consequent to pilocarpine-induced SE, by itself, accounts for the change in discharge behavior reported here. However, changes in expression of voltage-gated channels other than Ca²⁺ channels also may contribute to the intrinsic neuronal plasticity. Indeed, it was found previously (Sanabria et al., 2001), and confirmed in the present study, that some CA1 neurons in SE-experienced animals display a Ca²⁺-independent burst mechanism. A likely candidate for mediating Ca²⁺-insensitive bursting in CA1 pyramidal cells is the persistent Na⁺ current (Azouz et al., 1996; Su et al., 2001), but the contribution of this current to SE-induced intrinsic plasticity has yet to be demonstrated.

Molecular basis of intrinsic neuronal plasticity

Our data allow us to propose that of the three known T-type Ca²⁺ channel ₁ subunits (i.e., _1H, _1I, and _1G), _1H most probably underlies the augmented T-type Ca²⁺ current and associated intrinsic bursting after pilocarpine-induced SE. It was shown that when expressed in human embryonic kidney cells, the Ca²⁺ currents mediated by the three cloned ₁ subunits are differentially blocked by Ni²⁺, with the _1H subunit being ~20-fold more sensitive (IC₅₀ values, 12 µM) than _1G and _1I subunits (IC₅₀ values, 250 and 216 µM, respectively) (Lee et al., 1999b). The T-type Ca²⁺ currents in CA1 pyramidal cells in both control and SE-experienced animals were highly sensitive to Ni²⁺ (IC₅₀ values of 24 and 28 µM, respectively), suggesting that _1H subunits contribute strongly to this current. Likewise, the slow (~4-5 msec) Ca²⁺ tail currents that follow mock action potentials suggest the involvement of _1H and/or _1G subunits, which have a comparably slow deactivation kinetics (Kozlov et al., 1999). Clearly, more experiments will be required to prove unequivocally the role of the _1H Ca²⁺ channel subunit in SE-induced intrinsic plasticity. Interestingly, it was shown recently that intrinsic bursting in thalamic neurons relies on expression of the _1G subunit (Kim et al., 2001); thus intrinsic bursting in different classes of neurons may be produced by distinct T-type Ca²⁺ channel subunits.

Functional consequences of altered intrinsic neuronal properties

Modifications of intrinsic neuronal properties dependent on neuronal activity have been described previously in invertebrate (Turrigiano et al., 1994) and vertebrate (Desai et al., 1999) culture models. In these studies, long-term deprivation of activity causes neurons to fire more rapidly in response to injected current (Desai et al., 1999) or even to switch from a tonic to a burst firing mode (Turrigiano et al., 1994). Such mechanisms are thought to be homeostatic, i.e.,. they serve to stabilize the properties of neural circuits (Stemmler and Koch, 1999; Turrigiano, 1999). The plasticity that we describe here represents the converse: SE produces a long-lasting gain in the input-output properties of CA1 neurons. Increased bursting is observed up to 90 d after status epilepticus (our unpublished data), suggesting that this form of plasticity may be stable over prolonged periods of time.

Computer modeling studies of realistic neuronal networks have previously suggested that intrinsic bursters are pivotal in the generation of epileptiform activity (Traub and Wong, 1982; Miles and Wong, 1983). There is also a large body of experimental evidence in support of this contention. Increased intrinsic bursting is observed in acute models of hippocampal epilepsy, such as the high-K⁺ model (Jensen et al., 1994, 1996; Azouz et al., 1996, 1997; Su et al., 2001). Moreover, intrinsic bursters were shown to be the forerunners of epileptiform events in vitro, suggesting that they may be important in initiating epileptiform discharges (Chagnac-Amitai and Connors, 1989; Jensen and Yaari, 1997; Sanabria et al., 2001). Therefore, identification of the mechanisms responsible for the abnormal intrinsic bursting in epileptic tissue may permit pharmacological inhibition of seizure initiation in experimental and human epilepsy. It should be noted, however, that an episode of SE induced by pilocarpine or other procedures triggers long-term changes in synaptic function that may also play a role in the development of an epileptic condition (McNamara, 1999).

In summary, our observations suggest that the transformation of CA1 pyramidal cells from regular firing to burst-firing after pilocarpine-induced SE involves the persistent augmentation of a T-type Ca²⁺ current, possibly that mediated by the _1H subunit. This SE-induced intrinsic plasticity leads to a marked change in the input-output properties of hippocampal neurons that, in concert with altered synaptic connectivity, may underlie the hyperexcitability characteristic of TLE. Furthermore, these results suggest that subunit-selective T-type Ca²⁺ channel blockers may be promising targets for rational anti-epileptic drug design in TLE.

	FOOTNOTES

Received Dec. 17, 2001; revised Feb. 11, 2002; accepted Feb. 18, 2002.

^* H.S. and D.S. contributed equally to this work.

This research was supported by the German-Israel collaborative research program of the Ministry of Science and the Bundesministerium für Bildung und Forschung, Deutsche Forschungsgemeinschaft EL 122/7, the SFB 6006, the Israel Science Foundation, a University of Bonn Medical Center "BONFOR" grant, the Erna D. and Henry J. Leir Chair for Research in Neurodegenerative Diseases, and a Humboldt Research Award to Y.Y. We thank E. Perez-Reyes, T. Schneider, and A. Konnerth for critical comments.

Correspondence should be addressed to Dr. Heinz Beck, Department of Epileptology, University of Bonn Medical Center, Sigmund-Freud Strasse 25, D-53105 Bonn, Germany. E-mail: heinz.beck{at}ukb.uni-bonn.de.

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