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Department of Physiology and Biophysics, College of Medicine, University of Illinois at Chicago, Chicago, Illinois
Submitted 13 March 2006; accepted in final form 3 September 2006
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ABSTRACT |
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 TOP ABSTRACT INTRODUCTIONMETHODSRESULTSDISCUSSIONGRANTSACKNOWLEDGMENTSREFERENCES |
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INTRODUCTION |
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TOPABSTRACTINTRODUCTIONMETHODSRESULTSDISCUSSIONGRANTSACKNOWLEDGMENTSREFERENCES |
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). Earlier behavioral and pharmacological studies showed that the mesolimbic dopamine pathway is critical for the reinforcing effects of ethanol (Appel et al. 2004; DiChiara and Imperato 1988; Weiss et al. 1993). Pharmacological study with dopamine agonists and antagonists also supports the involvement of dopamine in ethanol reinforcement (Samson et al. 1990). It was previously reported that rats self-administer ethanol directly into the VTA (Rodd-Henricks et al. 2000) and ethanol excites dopamine cells in the VTA (Gessa et al. 1985). Thus ethanol-induced excitation of DA VTA neurons would increase dopamine release in the NAcb and mediate the reinforcing effects of ethanol.
There are many studies on the ethanol modulation of ligand-gated ion channels in central neurons. In hippocampal neurons, N-methyl-D-aspartic acid (NMDA)-receptor–mediated current is inhibited by ethanol (Hendricson et al. 2004; Lovinger et al. 1989; Peoples and Weight 1995). 
-Aminobutyric acid type A (GABAA)-receptor–mediated response is potentiated by ethanol in hippocampal neurons (Aguayo and Pancetti 1994; Proctor et al. 1992). Glycine-receptor–mediated response is potentiated by ethanol in midbrain dopamine neurons (Ye et al. 2001) and hypoglossal motoneurons (Eggers and Berger 2004). Adenosine (P2X) receptor–mediated current is inhibited by ethanol in hippocampal neurons (Li et al. 2000). Although ethanol modulates ligand-gated ion channels and affects the excitability of central neurons, the effect of ethanol on modulation of voltage-dependent ion channels in the CNS has not been well studied. DA VTA neurons have intrinsic pacemaker activity with the average firing frequency of 0.5–5 Hz and several voltage-dependent ionic currents contribute to the excitability of these neurons (Appel et al. 2003, 2006; Brodie and Appel 1998; Brodie et al. 1990, 1999; Koyama and Appel 2006a,b; Koyama et al. 2005; Mueller and Brodie 1989; Neuhoff et al. 2002; Okamoto et al. 2006). Therefore the effects of ethanol on voltage-dependent ion channels and the subsequent change in the excitability of these neurons are important cellular mechanisms involved in the reinforcing effects of ethanol.
We previously reported that ethanol increases the spontaneous firing frequency of acutely dissociated DA VTA neurons, in which the influence of synaptic activity on the excitability of these neurons was eliminated (Brodie et al. 1999). Our current-clamp studies suggest that ethanol excites DA VTA neurons by reducing a K+ current, which contributes to the action potential (AP) afterhyperpolarization (AHP) (Appel et al. 2003; Brodie and Appel 1998). In addition, our voltage-clamp studies showed that ethanol reduces the sustained K+ currents of DA VTA neurons (Appel et al. 2003; Brodie et al. 2000). Thus it is likely that ethanol excites DA VTA neurons directly by the reduction of K+-channel conductance.
M-current (IM) is a sustained K+ current and activated at the subthreshold range of membrane potential, regulating AP generation (Aiken et al. 1995; Brown and Adams 1980). Five types of KCNQ (KCNQ1–5) channels were previously reported to mediate IM (Lerche et al. 2000; Selyanko et al. 2000; Shapiro et al. 2000; Sogaard et al. 2001; Wang et al. 1998). Immunohistochemical co-localization of KCNQ2 and KCNQ4 channel subunit proteins was previously found in VTA neurons (Cooper et al. 2001; Kharkovets et al. 2000). We recently showed that IM regulates action potential generation to reduce the excitability by underlying fast and slow AHP components without changing the middle component of AHP (Koyama and Appel 2006a). Consistent with this finding, it was earlier shown that the KCNQ4 channel subunit is the major KCNQ subunit in DA VTA neurons and regulates the excitability of these neurons (Hansen et al. 2006). Interestingly, Moore et al. (1990) showed that ethanol reduces IM in CA1 hippocampal pyramidal neurons.
In our present study, we examined whether ethanol inhibition of IM contributed to the excitation of DA VTA neurons. For this purpose, we used acutely dissociated VTA neurons with enzyme treatment, in which both excitatory and inhibitory synaptic influences on these neurons were eliminated (Koyama et al. 2005) and nystatin-perforated patch recording to minimize intracellular dialysis and prevent the rundown of IM (Koyama and Appel 2006a). Part of this work previously appeared in abstract form (Koyama and Appel 2004).
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METHODS |
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TOPABSTRACTINTRODUCTIONMETHODSRESULTSDISCUSSIONGRANTSACKNOWLEDGMENTSREFERENCES |
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Animals used in this study were treated in strict accordance with the U.S. National Institutes for Health Guide for the Care and Use of Laboratory Animals and all experimental methods were approved by the Animal Care Committee of the University of Illinois at Chicago. Each Fisher 344 rat (14–18 days old) was decapitated and the brain quickly removed. The brain was placed in the ice-cold cutting solution consisting of (in mM): 220 sucrose, 2.5 KCl, 2.4 CaCl2, 1.3 MgSO4, 1.24 NaH2PO4, 26 NaHCO3, and 11 D-glucose, which was constantly bubbled with 95% O2-5% CO2. Transverse brain slices, at a thickness of 400 µm, were made using a Vibratome. The brain slices were incubated for 30 min in artificial cerebrospinal fluid (ACSF), consisting of (in mM): 126 NaCl, 2.5 KCl, 2.4 CaCl2, 1.3 MgSO4, 1.24 NaH2PO4, 26 NaHCO3, and 11 D-glucose (osmolarity 300 mosM), which was constantly bubbled with 95% O2-5% CO2 at room temperature (23–25°C). The brain slices were then incubated in a HEPES-buffered solution (in mM: 145 NaCl, 2.5 KCl, 2 CaCl2, 1 MgCl2, 10 HEPES, and 11 D-glucose (pH adjusted to 7.4 with NaOH; osmolarity, 300 mosM) containing papain (15–18 U/ml) at 32°C for 20–25 min. After papain treatment, the brain slices were further incubated in the ACSF for 20–40 min. The VTA neurons were dissociated using a vibrating stylus apparatus dispersing cells from the brain slices as previously described (Koyama et al. 2005). Once the cell dissociation procedure was completed (4–7 min), the brain slice was removed from the culture dish and the dissociated neurons settled and adhered to the bottom of the dish within 20 min. The dissociation procedure with papain described above was earlier shown to yield acutely dissociated VTA neurons (Koyama et al. 2005) and no spontaneous synaptic potentials or synaptic currents were recorded from these neurons in the present study. DA VTA neurons were identified in current-clamp recording based on electrophysiological characteristics previously described (Koyama and Appel 2006a).
Nystatin-perforated patch recording in dissociated neurons
Electrophysiological measurement was performed using an Axopatch-1B patch-clamp amplifier (Axon Instruments, Union City, CA). The tip resistances of the electrodes ranged from 1 to 2.5 M
when filled with pipette solution (in mM: 60 K-acetate, 60 KCl, 1 CaCl2, 2 MgCl2, and 40 HEPES; pH adjusted to 7.2 with KOH; final [K+]i = 131 mM; osmolality, 290 mOsm). To minimize the rundown of IM, nystatin-perforated patch recording was used as previously described (Koyama and Appel 2006a). Nystatin was dissolved in methanol at a concentration of 10 mg/ml. This nystatin stock solution was diluted with pipette solution to a final concentration of 100–200 µg/ml and the electrodes were backfilled with this solution. After cell-attached configuration had been completed, access resistance was periodically monitored and capacitative transients were cancelled. When the access resistance had reached a steady level (8–14 M), the recording was started. Completion of perforated patch was distinguished from membrane rupture because the hallmark of membrane rupture was accompanied by the sudden appearance of steep capacitative transients with the reduction of access resistance to 3–7 M; this can be compared with the access resistance in conventional whole cell configuration, described previously (Koyama and Appel 2006b). Pore formation with the nystatin-perforated patch technique is not accompanied by steep capacitance transients. Current- and voltage-clamp recordings were carried out with the HEPES-buffered solution constantly bubbled with 100% O2. The liquid junction potential between the pipette solution and the HEPES-buffered solution was estimated to be 5 mV (Neher 1992) and the results were corrected. Membrane currents and voltages were filtered at 1 kHz and acquired at a sampling frequency of 10 kHz. Data acquisition was performed by a DigiData 1322A interface and pClamp software version 9.0 (Axon Instruments). The dissociated VTA neurons were visualized under phase-contrast on an inverted microscope (Diaphot 300, Nikon, Tokyo, Japan). All experiments were performed at room temperature (23–25°C).
Drug application for dissociated neurons
Neurons were continuously bathed in control HEPES-buffered solution and drugs were dissolved at a final concentration in the same solution. Drug solutions were applied by a multiple channel manifold (Becton Dickinson). Each channel of the manifold was connected to a gravity-fed reservoir with tubing (ID 860 µm). The output of the manifold was connected to an outflow tube (ID 580 µm), the tip of which was placed within 200 µm of the soma of the recorded neuron. Solution flowed continuously through one manifold channel. Application of drug solutions was controlled by opening or closing valves connected to the reservoirs. The behaviorally active range of blood ethanol concentrations in the rat extends from 40 mM (sedation) to 90 mM (loss of righting reflex) (Majchrowicz and Hunt 1976); the lethal blood ethanol concentration in rats is about 200 mM (LD50 = 202 mM) (Haggard et al. 1940). Rats self-administer 44–55 mM ethanol directly into the VTA, indicating that this concentration of ethanol is reinforcing in the whole animal (Rodd-Henricks et al. 2000). In the present study, we examined ethanol concentrations in the range of 20 to 120 mM, which are pharmacologically relevant and sublethal concentrations in the rat.
Preparation of brain slices
After rapid removal of the brain, the tissue block containing the VTA was mounted in the Vibratome and submerged in the ice-cold cutting solution. Coronal sections (400 µm thick) were cut and the slice was placed on a mesh platform in the recording chamber. The slice was totally submerged in the ACSF maintained at a flow rate of 2 ml/min; the temperature in the recording chamber was kept at 35°C. The ACSF was saturated with 95% O2-5% CO2 (pH = 7.4). Equilibration time of 
1 h was allowed after placement of the brain slice in the recording chamber before electrodes were placed in the tissue. Recording electrodes were placed in the VTA under visual control. Only those neurons that were anatomically located within the VTA and that conformed to the electrophysiological criteria for dopaminergic neurons (Mueller and Brodie 1989) were studied. These criteria include broad action potentials and regular spontaneous firing frequency at 0.5–5 Hz.
Extracellular recording in brain slices
Extracellular recording electrodes were fabricated from 1.5-mm-diameter glass tubing and were filled with 0.9% NaCl. Tip resistance of the microelectrodes ranged from 3 to 8 M. The amplifier (Fintronics, Orange, CT) used in these recordings includes a window discriminator, the output of which was fed to both a rectilinear pen recorder and a computer-based data acquisition system that was used for on-line and off-line analysis of the data. The multiplexed output of the amplifier was displayed on an analog storage oscilloscope, for accurate adjustment of the window levels used to monitor single units. An IBM PC–based data acquisition system was used to calculate, display, and store the frequency of firing over 5-s and 1-min intervals.
Drug administration for brain slices
Drugs were added to the ACSF by means of a calibrated infusion pump from stock solutions 100- to 1,000-fold the desired final concentrations. The addition of drug solutions to the ACSF was performed in such a way as to permit the drug solution to mix completely with the ACSF before this mixture reached the recording chamber. The use of a calibrated, variable-speed infusion pump permits the accurate addition of several concentrations of drugs from the same stock solution. Final concentrations were calculated from the ACSF flow rate, pump infusion speed, and the concentration of drug stock solution. The small volume chamber (about 300 µl) used in this study permitted the rapid application and washout of drug solutions. Drugs typically reached equilibrium in the tissue after 2 to 3 min of application. A stock solution of 95% ethanol was used in the pump and infusion of ethanol never exceeded 1% of the flow rate of the ACSF.
Drugs and chemical agents
Dimethyl sulfoxide (DSMO), ethanol, HEPES, and nystatin were purchased from Sigma–Aldrich (St. Louis, MO). Papain was purchased from Worthington (Lakewood, NJ). 10,10-Bis(4-pyridinyl-methyl)-9(10H)-anthracenone (XE991) dihydrochloride was purchased from Tocris-Cookson (Ellisville, MO).
Data analysis
Action potentials were analyzed off-line by pClamp software (version 9.0, Axon Instruments). Interspike interval (ISI) histograms were created as previously described (Cocatre-Zilgien and Delcomyn 1992). The number of bins was equal to the square root of the number of ISIs. Bin width was obtained by dividing the ISI range (maximum ISI minus minimum ISI) by the number of bins. To assess the changes of spontaneous firing with drugs, drug effect was quantitated as the mean change in firing rate (normalized as the percentage of control) for a 60-s-long interval during the peak of the drug response as previously described (Brodie et al. 1990). The formula for this normalization is
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RESULTS |
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TOPABSTRACTINTRODUCTIONMETHODSRESULTSDISCUSSIONGRANTSACKNOWLEDGMENTSREFERENCES |
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As illustrated in Fig. 1, IM of DA VTA neurons was recorded in nystatin-perforated patch voltage-clamp configuration, with which IM is stably recorded without rundown. IM was measured in the standard deactivation protocol (Brown and Adams 1980) with 1-s-long hyperpolarizing voltage step from a holding potential (VH) of –25 to –40 mV. Ethanol at concentrations of 40, 80, and 120 mM reduced IM amplitude as well as the negative shift of the baseline outward current in DA VTA neurons (Fig. 1, A1–A3). Figure 1B shows the measurement of the inward relaxation current caused by deactivation of IM during the voltage step. IM amplitude was 32 pA in control and ethanol (120 mM) decreased IM amplitude to 20 pA.
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We then examined whether ethanol inhibition of IM was voltage dependent. Figure 3A shows IM induced by a series of hyperpolarizing voltage steps before, during, and after treatment with 120 mM ethanol. Ethanol inhibited IM measured with all four hyperpolarizing voltage steps in seven DA VTA neurons. Each IM in Fig. 3A was obtained by averaging the currents from the seven DA VTA neurons. Figure 3B shows the relationship between membrane voltage and normalized IM amplitude before (open circles), during (filled circles), and after (open triangles) treatment with 120 mM ethanol in the seven DA VTA neurons. The average normalized IM amplitude at –45 mV was 108.1 ± 2.1% in control, 74.2 ± 5.7% in the presence of 120 mM ethanol, and 92.3 ± 9.3% after washout of ethanol. Ethanol significantly reduced normalized IM amplitude (one-way ANOVA, F = 6.9, P < 0.01) but there was no significant difference in normalized IM amplitude between control and washout values (Student–Newman–Keuls post hoc test, P > 0.05). Figure 3C shows the relationship between membrane voltage and mean percentage inhibition of IM by 120 mM ethanol from the same seven DA VTA neurons. The average ethanol inhibition of IM obtained with each voltage was 27.3 ± 3.0% at –35 mV, 31.4 ± 4.9% at –45 mV, 31.9 ± 7.1% at –55 mV, and 31.3 ± 4.4% at –65 mV. There was no correlation between membrane voltage and IM inhibition rate by ethanol (r = –0.76, P > 0.2).
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In nystatin-perforated patch current-clamp recording, we examined the effect of ethanol on the spontaneous firing of DA VTA neurons. Ethanol (40 mM) increased firing frequency and this ethanol effect was reversible (Fig. 4A1). Figure 4A2 shows the time course of the effect of 40 mM ethanol on spontaneous firing. The effect of 40 mM ethanol on firing frequency for 60-s-long continuous recording was analyzed by an interspike interval (ISI) histogram (see METHODS) (Fig. 4A3); the distribution of ISI is shifted slightly leftward. Ethanol (80 mM) increased firing frequency and this ethanol effect was also reversible (Fig. 4B1). Figure 4B2 shows the time course of the effect of 80 mM ethanol on spontaneous firing. The effect of 80 mM ethanol on firing frequency was analyzed by the ISI histogram (Fig. 4B3); the distribution of ISI is shifted leftward. As shown in Fig. 4C, ethanol increased the firing frequency of DA VTA neurons in a concentration-dependent manner. Average ethanol-induced increase in firing frequency at each concentration was 6.5 ± 1.0% by 20 mM ethanol (n = 5), 11.4 ± 3.1% by 40 mM ethanol (n = 6), and 26.8 ± 4.9% by 80 mM ethanol (n = 10). From the graph in Fig. 4C, 20% increase in spontaneous firing frequency by ethanol was estimated to be produced by 60 mM. Among 14 DA VTA neurons, 120 mM ethanol increased firing frequency by 13.9 ± 2.6% in seven neurons (50%) and prevented spontaneous firing accompanied with membrane depolarization (depolarization inhibition) in seven neurons (50%). Therefore we did not include the results by 120 mM ethanol in this study.
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We next examined how IM inhibition contributes to the spontaneous firing of DA VTA neurons. For this purpose, we used a specific KCNQ channel inhibitor, XE991 (Wang et al. 1998). XE991 (1 µM) increased spontaneous firing frequency (Fig. 5A1). Figure 5A2 shows the time course of the effect of 1 µM XE991 on spontaneous firing. The effect of 1 µM XE991 on firing frequency was analyzed by the ISI histogram (Fig. 5A3); the distribution of ISI is shifted leftward. XE991 (10 µM) increased spontaneous firing frequency, an effect that was reversible (Fig. 5B1). Figure 5B2 shows the time course of the effect of 10 µM XE991 on spontaneous firing. The effect of 10 µM XE991 on firing frequency was analyzed by the ISI histogram (Fig. 5B3); the distribution of ISI is dramatically shifted leftward. As shown in Fig. 5C, XE991 increased the firing frequency of DA VTA neurons in a concentration-dependent manner. Average XE991-induced increase in firing frequency at each concentration was 8.7 ± 2.7% by 0.3 µM XE991 (n = 7), 23.6 ± 6.7% by 1 µM XE991 (n = 7), 42.0 ± 8.2% by 3 µM XE991 (n = 6), and 47.4 ± 7.4% by 10 µM XE991 (n = 8). Among 11 DA VTA neurons, 30 µM XE991 increased firing frequency by 62.1 ± 15.8% in seven neurons (64%) and completely prevented action potential generation accompanied with membrane depolarization in four neurons(36%). Therefore we did not include the results using 30 µM XE991 in this study.
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The question remained whether ethanol-induced reduction of IM could fully account for ethanol-induced excitation of DA VTA neurons. Our previous study showed that 0.3, 1, 3, and 10 µM XE991 reduced IM amplitude by 27.2 ± 3.8, 51.4 ± 2.9, 81.4 ± 1.7, and 86.6 ± 2.5% in DA VTA neurons (Koyama and Appel 2006a). By comparing the effect of XE991 on IM inhibition in the previous study and the effect of XE991 on firing frequency shown in Fig. 5C, we found a positive correlation between IM inhibition and increase in the firing frequency of DA VTA neurons produced by XE991 (Fig. 6A, open circles). The slope of the linear relationship was 0.5. In addition, we compared IM inhibition by ethanol shown in Fig. 2B and the increase in firing frequency produced by ethanol shown in Fig. 4C. In the same manner, we obtained a positive correlation between IM inhibition by ethanol and ethanol-induced increase in the firing frequency of DA VTA neurons (Fig. 6A, filled circles). The slope of this linear relationship for ethanol effects was 1.3.
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Extracellular single-unit recording was used to measure the effect of ethanol (40, 80, and 120 mM) on the firing frequency of DA VTA neurons in brain slices. After washout of the last concentration of ethanol, 10 µM XE991, a concentration that blocked IM by 87% (Koyama and Appel 2006a), was applied and the same concentrations of ethanol were tested again. The percentage increase in firing frequency produced by each ethanol concentration was calculated with the formula shown in METHODS. Figure 7 shows the concentration–response relationship between ethanol and the percentage increase in firing frequency by ethanol before and after treatment with 10 µM XE991 from 15 DA VTA neurons. The ethanol excitation was concentration dependent (P < 0.001). Before XE991 treatment, average ethanol-induced increase in firing frequency at each concentration was 11.2 ± 1.2% by 40 mM ethanol, 20.8 ± 2.2% by 80 mM ethanol, and 30.4 ± 3.0% by 120 mM ethanol (Fig. 7, filled circles). After treatment with 10 µM XE991, average ethanol-induced increase in firing frequency at each concentration was 10.4 ± 1.6% by 40 mM ethanol, 17.7 ± 1.9% by 80 mM ethanol, and 27.9 ± 4.8% by 120 mM ethanol (Fig. 7, filled squares). Although we anticipated the partial reduction of ethanol-induced excitation in the presence of 10 µM XE991, there was no statistically significant effect of XE991 on the ethanol concentration–response curve (P > 0.05). For the 15 DA VTA neurons, 10 µM XE991 produced no significant change of firing frequency (1.3 ± 1.5%).
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DISCUSSION |
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TOPABSTRACTINTRODUCTIONMETHODSRESULTSDISCUSSIONGRANTSACKNOWLEDGMENTSREFERENCES |
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showed that ethanol reduces IM amplitude in CA1 hippocampal pyramidal neurons. However, ethanol reduced IM more potently in that study than in the present report. Moore et al. (1990) reported that 44 mM ethanol reduces IM by 36%. Our present study shows that 120 mM ethanol reduces IM by 30%. The difference may have arisen from the types of KCNQ channels expressed in the hippocampus and the VTA. In the hippocampal CA1 region, KCNQ2, KCNQ3, and KCNQ5 channel subunit proteins were reported to be present (Shah et al. 2002). In the VTA, on the other hand, KCNQ2 and KCNQ4 channel subunit proteins were reported to be present (Cooper et al. 2001; Kharkovets et al. 2000). Our previous study suggests that KCNQ2 and KCNQ4 channel subunits are involved in DA VTA neurons by the analysis of pharmacological properties of IM (Koyama and Appel 2006a). A recent study reported that KCNQ4 channel subunit is the major KCNQ subunit in DA VTA neurons and regulates the excitability of these neurons (Hansen et al. 2006). We also found that ethanol inhibition of IM was not voltage dependent, suggesting that the ethanol action site is different from the voltage-sensitive regions of M-channels. This is consistent with other reports indicating that IM inhibition by some drugs of abuse such as ethanol (Moore et al. 1990) and cannabinoids (Schweitzer 2000) does not appear to be voltage dependent.
In nystatin-perforated patch current-clamp recording, 20–80 mM ethanol increased the firing frequency of DA VTA neurons in a concentration-dependent manner. These results are consistent with our previous study using dissociated DA VTA neurons (Brodie et al. 1999). In the present study, we found that ethanol at a concentration of 120 mM prevented spontaneous firing by depolarization inhibition in 50% of DA VTA neurons (at room temperature). In our previous study performed at 34°C, depolarization blockade was not observed in dissociated DA VTA neurons (Brodie et al. 1999). We reported that higher concentrations of ethanol (>300 mM) produce initial increases in firing frequency followed by the complete block of firing in DA VTA neurons (depolarization inhibition) (Appel et al. 2006). There is a possibility that the ethanol-induced depolarization inhibition of spontaneous firing in DA VTA neurons may depend on the temperature of bathing solutions. However, the cellular mechanism of the depolarization inhibition by ethanol in these studies is unclear and additional studies will be needed to elucidate how ethanol produces depolarization inhibition.
Treatment with XE991 increased firing frequency in a concentration-dependent manner in DA VTA neurons. The increase in the spontaneous firing frequency of DA VTA neurons produced by XE991 correlated positively with IM inhibition. This result suggests that IM plays a role in maintaining the spontaneous firing frequency of DA VTA neurons. From the linear relationship obtained with XE991, the contribution of IM inhibition by 80 mM ethanol is estimated to cause a 6% increase in the spontaneous firing frequency, given that 80 mM ethanol inhibited IM by 15%. The ethanol-induced increase in the spontaneous firing frequency of DA VTA neurons also correlated positively with IM inhibition by ethanol. However, we found a difference in the slope values for the linear relationship of IM inhibition versus increase in spontaneous firing frequency between ethanol (1.3) and XE991 (0.5). In addition, the 20% increase in spontaneous firing frequency by ethanol was obtained at 60 mM, which was smaller than the ethanol concentration that produced 20% inhibition of IM amplitude (90 mM). Furthermore, in the pharmacological occlusion experiment using the submaximal concentration of XE991, ethanol still increased the spontaneous firing frequency of DA VTA neurons in a concentration-dependent manner. These observations suggest that if ethanol inhibition of IM underlies excitation of DA VTA neurons, other additional ethanol effects on these neurons increase the magnitude of the effect of IM reduction on firing rate. Although we anticipated the partial reduction of ethanol-induced excitation in the presence of XE991, there was no statistically significant effect of XE991 on the ethanol concentration–response curve. Because 10 µM XE991 inhibits IM amplitude by 87% (Koyama and Appel 2006a) and this XE991 effect could increase the membrane input resistance, additional ethanol-induced excitatory effects on DA VTA neurons may be amplified through the increase in the membrane input resistance and compensating for the reduction of the contribution of ethanol-induced IM inhibition to spontaneous firing frequency. It is noted that dissociated DA VTA neurons were more excited by ethanol and the block of IM than DA VTA neurons in brain slices. For example, 80 mM ethanol-induced increase in spontaneous firing frequency was 27% in dissociated neurons and 21% in neurons from brain slices. The XE991 (10 µM)–induced increase in spontaneous firing frequency was 47% in dissociated neurons and 1.3% in neurons from brain slices. Because dissociated DA VTA neurons were truncated from distal dendrites, the elimination of K+ conductance in distal dendrites presumably causes the dissociated neurons to be more excitable than the neurons in brain slices.
It is possible that ethanol may inhibit the other types of sustained K+ currents rather than IM in DA VTA neurons. We previously showed that 10 mM tetraethylammonium (TEA) blocks IM amplitude by 98% in DA VTA neurons (Koyama and Appel 2006a) and ethanol can still increase the spontaneous firing frequency of these neurons in the presence of 10 mM TEA (Appel et al. 2003). We also showed that ethanol-induced excitation of DA VTA neurons is blocked by a low concentration of quinidine (20–40 µM) (Appel et al. 2003). Thus ethanol may inhibit a quinidine-sensitive and relatively TEA insensitive sustained K+ current in addition to its inhibition of IM in DA VTA neurons. The candidates for the sustained K+ current are three different K+ channel families: Kv1 channels (Grissmer et al. 1994; Yeola et al. 1996), ether-a-go-go (eag) channels (Ludwig et al. 1994; Schonherr et al. 2002), and TASK channels (Leonoudakis et al. 1998; Meadows and Randall 2001). It is also possible that other ion channels such as Ih (Okamoto et al. 2006) could also play a role in ethanol excitation (but see Appel et al. 2003). The data of the present study taken together indicate that, although ethanol causes inhibition of IM and this results in some increase in firing frequency, another effect of ethanol is primarily responsible for the ethanol-induced increase in firing rate. Physiological reduction of this other predominantly ethanol-sensitive current (by neurotransmitter-mediated second-messenger events for example) could increase the relative importance of IM in firing of DA VTA neurons.
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ACKNOWLEDGMENTS |
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Present address of S. Koyama: Department of Pharmaceutical Care and Health Science, Fukuoka University, Fukuoka 814-0180, Japan.
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FOOTNOTES |
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Address for reprint requests and other correspondence: S. Koyama, Department of Physiology and Biophysics (M/C 901), University of Illinois at Chicago, 835 S. Wolcott Avenue, Chicago, IL 60612-7342
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