| HOME | HELP | FEEDBACK | SUBSCRIPTIONS | ARCHIVE | SEARCH | TABLE OF CONTENTS |
|
|
|
|||||||
|
|||||||||
| ||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||
1Department of Physiology and Biophysics, University of Alabama at Birmingham, Birmingham, Alabama; and 2 Department of Odontology and Oral Pathology, Faculty of Dentistry, Chiang Mai University, Chiang Mai, Thailand
Submitted 15 April 2005; accepted in final form 21 December 2005
 |
ABSTRACT |
|---|
|
|
|
INTRODUCTION |
|---|
|
; Sloviter 1987; Zhao and Leung 1991). In spinal cord and brain stem, strychnine-sensitive glycine-gated chloride channels (GlyRs), along with GABA-gated receptors (GABAARs), mediate potent inhibition. Elegant electrophysiological studies show that glycine and GABA are coreleased from interneuron terminals in both spinal cord and brain stem and simultaneously activate postsynaptic GlyRs and GABAARs (Chery and de Koninck 1999; Jonas et al. 1998; O'Brien and Berger 1999). Until recently, a potential role for inhibitory GlyRs in regions of the forebrain, including hippocampus, received little attention by investigators interested in inhibitory mechanisms, most likely because of the misconception that functional GlyR expression ceases early in development (Ito and Cherubini 1991; Malosio et al. 1991) and to studies showing that fast synaptic inhibition is completely abolished by GABAAR antagonists (Ito and Cherubini 1991; Mody 1998). It is now clear that GlyRs are functionally expressed in many brain regions including hippocampus, hypothalamus, amygdala, striatum, ventral tegmental area, substantia nigra, inferior colliculus, cerebellum, and cortex (Chattipakorn and McMahon 2002, 2003; Dumoulin et al. 2001; Hussy et al. 2001; Karkar et al. 2004; Kawa 2003; Mangin et al. 2002; McCool 2001; Sergeeva and Haas 2001; Xu et al. 2004; Ye et al. 1997, 1999, 2001), suggesting that neuronal inhibition in many, if not all, brain regions is mediated by both GABA and glycine-gated chloride channels.
The precise function of GlyRs among these brain regions is not yet clearly defined, and in many regions, GlyRs are believed to be located only at extrasynaptic sites (Deleuze et al. 2005; Flint et al. 1998; Mangin et al. 2002; Wang et al. 2005) where they could be important mediators of tonic inhibition similarly to the function of extrasynaptic GABAARs (Farrant and Nusser 2005; Mori et al. 2002; Petrini et al. 2004) and provide critical neuroprotection under pathological conditions when extracellular glycine and taurine levels are elevated (Baker et al. 1991; Saransaari and Oja 1997, 1999; Zhao et al. 2005). In hippocampus, glycinergic synapses have been morphologically, but not functionally, defined at a small subset of synapses in dissociated hippocampal cultures and in slices (Danglot et al. 2004; Levi et al. 2004; Meier and Grantyn 2004). However, GlyRs have been shown to mediate fast synaptic transmission synapses in cerebellum, where glycine and GABA are coreleased from Golgi cells and activate postsynaptic GlyRs and GABAARs in either separate or mixed synapses depending on the target (Dugue et al. 2005; Dumoulin et al. 2001). More recently, inhibitory synaptic transmission in thalamus has been shown to be partially mediated by GlyRs (Ghavanini et al. 2005).
Previously, we have reported that CA1 pyramidal cells and GABAergic interneurons in stratum radiatum, as well as granule cells and hilar interneurons in the dentate gyrus, express functional GlyRs in mature hippocampal slices (Chattipakorn and McMahon 2002, 2003). However, little is known regarding the effects of GlyR activation on hippocampal excitability and synaptic circuits. In this study, we report that activation of GlyRs limits activity in the synaptic network by depressing suprathreshold excitatory postsynaptic potentials (EPSPs) to subthreshold events in recordings from both CA1 pyramidal cells and interneurons. Blockade of postsynaptic GlyRs or decreasing the driving force for chloride ions in the postsynaptic cell attenuates the depression. These findings suggest a postsynaptic locus for the depression, which likely involves a current shunt caused by the large GlyR-mediated decrease in postsynaptic input resistance (Rin). This GlyR-mediated depression of synaptic transmission we report here provides an additional inhibitory mechanism in hippocampus that will work together with other well-known GABAergic inhibitory mechanisms to control neuronal excitability. Using double immunohistochemical labeling, we show that GABAergic interneurons are immunopositive for the amino acid glycine as well as the glycine transporter, GlyT2, strongly suggesting that these cells are a source of glycine. The co-localization of glycine and GABA in hippocampal interneurons raises the interesting possibility that these neurons use both neurotransmitters, similar to interneurons in spinal cord, brain stem, and thalamus and golgi cells in cerebellum (Chery and de Koninck 1999; Dumoulin et al. 2001; Ghavanini et al. 2005; Jonas et al. 1998; O'Brien and Berger 1999), to provide critical inhibition required for normal hippocampal function.
|
|
METHODS |
|---|
|
Brain slice preparation
Experiments were performed on acutely prepared hippocampal slices (400 µM) obtained from 3- to 4-wk-old Sprague-Dawley rats. Slices were cut into ice-cold high sucrose and low calcium artificial cerebral spinal fluid (ACSF; in mM): 85 NaCl, 25 NaHCO3, 2.5 KCl, 1.25 NaH2PO4, 0.5 CaCl2, 4 MgSO4, 25 glucose, 0.5 ascorbate, 75 sucrose, and 2 kynurenic acid; saturated with 95% O2-5% CO2, pH 7.4. Slices were incubated for 30 min in a submersion chamber before being transferred to standard ACSF that included 1 mM kynurenic acid (in mM): 119 NaCl, 26 NaHCO3, 2.5 KCl, 1.0 NaH2PO4, 2.5 CaCl2, 1.3 MgSO4, and 10 glucose, saturated with 95% O2-5% CO2, pH 7.4. Slices were rested for an additional 30 min before being used in experiments. ACSF with or without kynurenic acid (as mentioned) was used for recordings. All experiments were performed in a submersion recording chamber with a constant flow rate of 4–5 ml/min and ACSF warmed to 27–28°.
Electrophysiological recordings
Whole cell voltage- and current-clamp recordings of visually identified CA1 pyramidal cells and GABAergic interneurons in s. radiatum were obtained using IR-DIC microscopy and standard recording techniques (Chattipakorn and McMahon 2002). An Axoclamp 2A or Axopatch 200 amplifier (Molecular Devices, Sunnyvale, CA) was used to amplify recorded signals, and responses were monitored on an oscilloscope and computer monitor. Patch electrodes had resistances between 4 and 6 M
when filled with (in mM) 110 cesium chloride or cesium gluconate, 0.6 EGTA, 5 MgCl2, 2 ATP-Na2, 3 GTP-Na, 40 HEPES, and 0.4% biocytin, pH 7.2, 260–270 mOsm. For current-clamp recordings, 110 mM potassium gluconate was substituted for cesium gluconate. In some recordings, 5 mM QX 314 was added to the internal solution to block voltage-dependent Na+ channels and to enhance space-clamp. In some experiments, the nonselective chloride channel blocker 4,4'-diisothiocyanatostilbene-2-2'-disulfonic acid (DIDS) was added to the pipette solution to block postsynaptic GlyRs. DIDS has been shown to block GlyRs (Leewanich et al. 1998) and has been used previously in the pipette solution to block postsynaptic GABAARs in hippocampal slices (Albertson et al. 1996; Hollrigel et al. 1998). Recorded neurons were identified as pyramidal or interneuron by their electrical properties (e.g., input resistance, firing pattern). Evoked synaptic events were elicited at 0.1 Hz through a bipolar stimulating electrode placed in s. radiatum. In addition, neurons were filled with 0.4% biocytin and processed to allow for post hoc neuronal identification (McMahon and Kauer 1997). No recorded interneurons were identified as radiatum giants (Maccaferri and McBain 1996).
Data were filtered at 3 kHz and acquired and analyzed using pCLAMP (Molecular Devices) and custom written software in Labview (Dr. Richard Mooney, Duke University). Cell input resistance (ranging from 120 to 180 M for pyramidal cells and 200 to 400 M for interneurons) and series resistance (11–18 M) were continually monitored throughout the recording, and recordings were terminated when these values increased by 
20%. Cell capacitance was monitored and recorded using the membrane test tool in pCLAMP. All data are reported as mean ± SE. Student's t-test was used to test for significance, and results were deemed significant at P < 0.05.
Drug delivery
Stock solutions of all agonists and antagonists were prepared in deionized distilled water with the exception of the GlyT1 inhibitor, N[3-(4'-fluorophenyl)-3-(4'phenylphenoxy)propyl]sarcosine (NFPS), which was dissolved in DMSO. All drugs were diluted to appropriate concentrations in the bathing solution. The glycine concentration (300 µM) used in this study was chosen because it is near the apparent glycine EC50 for these receptors in slices (Chattipakorn and McMahon 2002). In experiments examining the effects of GlyR activation on evoked synaptic transmission, glycine was applied by bath perfusion of a fixed concentration where complete bath exchange occurred within 1.5 min. During bath application of glycine, GlyR currents do not completely desensitize, even during prolonged agonist application, but reach a steady-state current (59 ± 10% of peak current in pyramidal cells; 47 ± 19% of the peak current in interneurons; Chattipakorn and McMahon 2002). In some experiments where the effects of antagonists or the interactions between currents mediated by GlyRs and other ligand-gated channels were being assessed, a small volume of agonist (glycine, GABA, and glutamate) was applied directly to the recorded cell through a glass pipette placed within 50 µm of the recorded cell. The agonists were applied for 3–30 s through rapid gravity flow using a multichannel valve or by pressure ejection using a picospritzer. This method allowed agonists to be applied repeatedly to a given cell and at short intervals.
Immunohistochemistry
Three- to 4-wk-old rats (n = 8) were anesthetized with pentobarbital sodium and perfused with ACSF followed by perfusion with cold 4% paraformaldehyde. Brains were postfixed in 4% paraformaldehyde for 2 h (except in the case of GlyR staining), cryoprotected in 30% sucrose, and resectioned (40 µm). In experiments using anti-GlyR antibodies, sections were permeabilized with methanol and washed with 0.1 M TBS-TX buffers. Primary antibodies used in this study included mouse anti-GlyR mAb4a (1:25; Connex), rabbit anti-glycine antibody (1:100), guinea pig anti-neuronal glycine transporter 2 (1:1,000; Chemicon), mouse anti-GABA (1:5; Chemicon), and rabbit anti-glutamic acid decarboxylase (GAD) 67 (1:500; Chemicon). Sections were incubated with appropriate Alexa-conjugated secondary antibodies (1:300; Molecular Probes), washed, mounted, and coverslipped. Controls were performed by eliminating the primary antibody from the reaction mixture. In double labeling experiments, sections were incubated with both primary antibodies simultaneously, followed by simultaneous incubation with appropriate secondary antibodies. Confocal microscopy was used to visualize stained cells.
|
|
RESULTS |
|---|
|
). In all experiments in this study, we used 300 µM glycine to activate GlyRs because this concentration is near to the EC50 for GlyRs expressed by both pyramidal cells and interneurons recorded in hippocampal slices (Chattipakorn and McMahon 2002). Here we show representative GlyR-mediated currents recorded in whole cell voltage-clamp conditions from a CA1 pyramidal cell (Fig. 1A, top) and a s. radiatum interneuron (Fig. 1A, bottom) after brief application of glycine (30 s, ECl– = 0 mV) through a drug pipette positioned within 50 µm of the recorded cell. The currents only partially desensitize and rapidly recover to baseline after termination of agonist application. These glycine-induced currents are mediated by GlyRs because they are relatively unaffected by the GABAA receptor (GABAAR) antagonist bicuculline (10 µM; although bicuculline has been shown to block GlyRs; Wang and Slaughter 2005), but are reversibly blocked by the GlyR antagonist strychnine (1 µM; IC50 20–40 nM; see Chattipakorn and McMahon 2002). With repeated glycine applications (30 s, 5-min intervals), GlyR-mediated current amplitude remains stable, indicating that GlyR channel function does not rundown during whole cell recordings (Fig. 1B). GlyR-mediated responses were observed in all recorded pyramidal cells and interneurons, but consistent with our previous report (Chattipakorn and McMahon 2002), the mean current amplitude and decrease in cell input resistance (Rin; measured at the peak of the current) are significantly larger in interneurons (1351 ± 138 pA and 77 ± 4% decrease in Rin, n = 7) than in pyramidal cells (820 ± 173 pA and 65 ± 3% decrease in Rin, n = 5; Fig. 1, C1 and C2; P < 0.05, pyramidal cells vs. interneurons). Comparison of GlyR current density (pA/pF) versus percent decrease in Rin shows, as expected, that larger currents are accompanied by larger changes in Rin (Fig. 1D), and furthermore, there is an overall larger current density measured in interneurons.
|
GlyRs are well-characterized mediators of neuronal inhibition in spinal cord and brain stem. Therefore we next tested, using whole cell current-clamp recordings from both pyramidal cells and interneurons, whether GlyR activation can depress somatically induced action potentials after direct depolarizing current injection through the patch pipette. In these experiments, we injected hyperpolarizing, subthreshold, threshold, and suprathreshold depolarizing current pulses in the absence and presence of glycine to determine GlyR-mediated effects on Rin and somatically generated action potential firing. Glycine was bath applied so that the effects of GlyR activation on action potential generation could be assessed after the current reached steady state. Although GlyR currents partially desensitize, there is a significant steady-state current (>50% of peak amplitude in both pyramidal cells and interneurons) maintained for the duration of glycine application (at least 
10 min, the longest we have measured; Chattipakorn and McMahon 2002). Importantly, there is no statistical difference in the amount of desensitization between pyramidal cells and interneurons (Chattipakorn and McMahon 2002).
Bath application of glycine (300 µM) elicited a modest depolarization, rather than hyperpolarization, of the membrane potential from the resting potential (pyramidal cells: resting potential, 69 ± 1 mV; GlyR-induced depolarization, 2 ± 1 mV, n = 5; interneurons: resting potential 70 ± 2 mV; GlyR-induced depolarization, 6 ± 1 mV, n = 6, P < 0.05 pyramidal cells vs. interneurons) that was accompanied by a significant decrease in Rin (measured during steady state rather than at the peak as in Fig. 1) in both cell types [Fig. 2, A and B, cf. amplitude of the downward deflection (blue traces) in left and middle; 33 ± 4% decrease in pyramidal cells, n = 5; 48 ± 5% decrease in interneurons, n = 6, P < 0.05 pyramidal cells vs. interneurons]. The glycine-induced depolarization of the membrane potential indicates that the chloride reversal potential is more depolarized than the resting potential, which is often the case for GABAAR-mediated currents (Jackson et al. 1999; Staley and Mody 1992). After washout, the change in membrane potential and Rin recovered to their original values. Similar to our findings in the voltage-clamp recordings, there is a larger decrease in Rin (and membrane potential depolarization) in interneurons compared with pyramidal cells.
|
GlyR activation depresses synaptically generated action potentials
Regulation of excitatory circuits is critical to normal hippocampal function. Therefore we next sought to determine whether GlyR activation could depress synaptically generated action potentials elicited by stimulation of excitatory synapses. We tested this idea by recording in whole cell current-clamp suprathreshold EPSPs generated through electrical stimulation of schaffer collateral afferents located in s. radiatum (0.1 Hz). In these experiments, we set our stimulus intensity to a minimum (threshold) value so that only one synaptically generated suprathreshold EPSP was evoked in the majority of trials. Within 1–2 min, bath perfusion of glycine (300 µM) reversibly depressed suprathreshold EPSPs to subthreshold events in both pyramidal cells (n = 9/10) and interneurons (n = 10/10; Fig. 3, A and B). This effect of glycine was prevented in the presence of 1 µM strychnine. Although suprathreshold EPSPs were depressed to subthreshold events in nearly all cells recorded (1 pyramidal cell had no effect), the magnitude of the depression was variable from cell to cell (Fig. 3, A2 and B2). In pyramidal cells, the percentage of trials generating suprathreshold EPSPs during glycine application was decreased by 22 ± 8% (n = 4) and by 27 ± 8% in interneuron recordings (n = 4; P > 0.37, pyramidal cells vs. interneurons). Because glycine application increases N-methyl-D-aspartate receptor (NMDAR)-mediated currents (Bergeron et al. 1998; Wilcox et al. 1996), we wondered whether a potential increase in NMDAR transmission was limiting the synaptic depression mediated by GlyRs. Therefore we tested whether the percentage of trials generating suprathreshold EPSPs would be further decreased in the presence of APV (100 µM) to block NMDARs. In pyramidal cells, the percentage of trials generating suprathreshold EPSPs was decreased by 32 ± 6% (n = 6). Although there is a trend toward a greater amount of depression when NMDARs are blocked, the values are not significantly different (P > 0.08). Similarly, in interneurons, the percentage of trials generating suprathreshold EPSPs was also not significantly different during blockade of NMDARs with APV compared with without the antagonist (33 ± 5% decrease in D-APV, n = 6, vs. 27 ± 8% without D-APV, n = 4, P > 0.25). In sum, our findings indicate that GlyR activation depresses synaptically driven action potentials in both pyramidal cells and interneurons, indicating the involvement of a general mechanism that affects both major cell types in hippocampus.
|
). Thus, the strychnine-mediated increase in excitability observed in the current-clamp recordings is likely caused by inhibition of GlyRs that are tonically open under basal conditions, although we cannot completely exclude some nonspecific effects of strychnine on other channels (Garcia-Colunga and Miledi 1999; Matsubayashi et al. 1998). Furthermore, because strychnine produced no measurable membrane potential depolarization or change in Rin measured at the soma, we speculate that the tonically active GlyRs are located in the dendrites at sites distant from the recording electrode where the voltage clamp is much less effective (Carnevale et al. 1997; Spruston et al. 1993). GlyR activation depresses the amplitude of evoked monosynaptic currents
There are several potential mechanisms that could underlie the GlyR-mediated depression of synaptically evoked suprathreshold EPSPs, including depression of glutamate release by presynaptic GlyRs (Turecek and Trussell 2001), facilitation of GABA transmission by presynaptic GlyRs (Ye et al. 2004), or a postsynaptic mechanism resulting from GlyR-mediated changes in membrane potential and Rin that could shunt incoming synaptic currents, similarly to GABAAR activation (Jackson et al. 1999; Staley and Mody 1992). To determine which mechanism(s) are responsible, we performed a series of experiments in voltage clamp where we measured changes in the amplitude of pharmacologically isolated AMPA receptor (AMPAR)-mediated EPSCs and GABAA receptor (GABAAR)-mediated IPSCs after GlyR activation. We limited our examination here to EPSCs mediated by AMPARs to simplify data interpretation because applied glycine can enhance NMDAR-mediated currents (Bergeron et al. 1998; Wilcox et al. 1996).
In voltage-clamp recordings, we found that activation of GlyRs by bath application of glycine (300 µM; CsCl pipette solution) elicited a >50% depression of both EPSCs (68 ± 15% n = 5 pyramidal cells; 64 ± 5% n = 10 interneurons) and IPSCs (52 ± 5%, n = 5 pyramidal cells; 64 ± 6%, n = 7 interneurons) that quickly recovered after washout (Fig. 4). The effect of glycine on EPSC and IPSC amplitude was prevented by strychnine (1 µM), showing the involvement of GlyRs. Interestingly, the amount of depression of EPSC and IPSC amplitude recorded from either cell type was not significantly different (P 0.42 for EPSC vs. IPSC depression in pyramidal cells and P 0.23 for the same comparison in interneurons), indicating that the mechanism causing the depression is not cell type specific and is not specific to a certain set of synapses. Rather, these findings indicate that the mechanism of depression is a general mechanism affecting all synapses on both cell types.
|
; Ye et al. 2004). To determine whether presynaptic GlyRs modulate glutamate release at schaffer collateral synapses, we examined the paired-pulse facilitation (PPF) ratio at CA3 synapses on pyramidal cells before and after bath application of glycine (300 µM). The PPF ratio (determined by dividing the amplitude of the second EPSC by the first when pairs of pulses are given at short intervals, here 50 ms) is an indirect measure of the initial release probability. An increase in this ratio during the course of an experiment is most often interpreted as a decrease in the release probability (Dobrunz and Stevens 1997; Kim and Alger 2001; Zucker 1989). However, we found that GlyR activation causes no change in the PPF ratio at glutamate synapses onto pyramidal cells (PPF ratio 1.9 ± 0.3 during baseline compared with 1.7 ± 0.2 during glycine, n = 5, P > 0.1, data not shown), indicating that the mechanism underlying the GlyR-mediated synaptic depression is most likely not presynaptic (Dobrunz and Stevens 1997; Kim and Alger 2001; Zucker 1989). Because CA3 synapses onto interneurons have a different release probability than those onto pyramidal cells (there is often paired-pulse depression or no change in transmission; Sun et al. 2005), examination of the paired-pulse ratio at interneuron synapses is not straight forward. Therefore given this issue, together with the lack of an effect on the PPF ratio at pyramidal cell synapses, we did not investigate this further.
Presynaptic GlyRs have been shown to increase, not decrease, GABAAR-mediated transmission (Ye et al. 2004). Therefore depression of the evoked IPSC amplitude is not likely mediated by presynaptic GlyRs. We considered the possibility that an alteration in ECl– during prolonged GlyR activation could be the mechanism. However, we observed no change in the reversal potential of currents mediated by exogenous application of GABA (300 µM, 3 s) in the presence of glycine compared with without glycine (ECl– = 0 mV; EGABA = 0.03 ± 0.06 mV in the absence and 0.01 ± 0.01 mV in the presence of glycine, P 0.3, n = 10, data not shown) indicating that ECl– has not been altered and therefore is not responsible for the GlyR-mediated depression of evoked GABAAR-mediated IPSCS.
GlyR-induced depression of synaptic transmission is mediated through a postsynaptic mechanism
The lack of a significant effect of GlyR activation on the PPF ratio during a >50% depression of the EPSC amplitude suggests that the GlyR-mediated depression of transmission is most likely not caused by presynaptic depression of neurotransmitter release. Also, because both EPSCs and IPSCs are depressed to the same degree in pyramidal cells and interneurons, we reasoned that the mechanism underlying the depression must be caused by a common postsynaptic mechanism that does not selectively affect excitatory or inhibitory synapses. We therefore investigated whether a postsynaptic locus is involved by performing several types of experiments. Because all of the results we have obtained thus far are common to both pyramidal cells and interneurons, the mechanism underlying the synaptic depression is likely to be the same between the cell types. Therefore to facilitate the study, we focused the next series of experiments on a single cell type and chose to concentrate on interneurons because GlyR responses are larger in these cells. However, as previously mentioned, because all of our findings thus far are the same between cell types, any conclusions reached in these experiments can most likely be extrapolated to pyramidal cells.
First, we reasoned that if the magnitude of the postsynaptic GlyR-mediated current contributed to the amount of depression of the synaptic events, changing the driving force for chloride in the postsynaptic cell should change the magnitude of the depression. We found that the depression of the EPSC amplitude is significantly less when recordings were performed with internal solution containing 10 mM chloride versus 110 mM chloride (Fig. 5, A and B; 17 ± 5% depression, Cs+ gluconate solution, ECl– = approximately –60 mV, n = 6 vs. 51 ± 4% depression, Cs+ chloride solution, ECl– = 0 mV, n = 5). As expected, the larger magnitude depression correlates with the larger postsynaptic GlyR-mediated current (146 ± 51 pA with Cs+ gluconate, n = 6, vs. 656 ± 152 pA with CsCl, n = 5; P < 0.05). Although the magnitude of the depression (and GlyR-mediated postsynaptic current) is much less using 10 mM intracellular chloride (Cs+gluconate pipette solution), the amplitude of the EPSC is significantly depressed from baseline during glycine application (P < 0.05).
|
; Saransaari and Oja 1998) in the pipette solution should prevent the effects of glycine on AMPAR currents, both synaptically evoked and elicited through exogenous agonist application. Note that because including DIDS in the pipette solution blocks GABAARs (Albertson et al. 1996; Hollrigel et al. 1998), GlyR-mediated effects in these experiments are limited to the examination of AMPAR-mediated responses.
Indeed, we found that pharmacologically isolated AMPAR and GABAAR currents elicited by brief application of glutamate (100 µM, 3 s) and GABA (50 µM, 3 s), respectively, were depressed (42 ± 5%, n = 5, and 50 ± 4%, n = 5, respectively; Fig. 6, A1 and A2) by bath perfusion of glycine (300 µM, CsCl pipette solution) during blockade of synaptic transmission with TTX (1 µM). In the next set of experiments, postsynaptic GlyRs were blocked by including DIDS in the pipette solution to test whether the effects of GlyR activation on the amplitude of AMPAR-mediated currents was prevented. First we confirmed that DIDS was able to block GlyRs and found that within 10–15 min of whole cell recording, GlyR-mediated currents were depressed nearly 80% (Fig. 6B1, n = 6). The depression of the GlyR currents with DIDS in the pipette solution cannot be explained by a nonspecific rundown of GlyR currents because we showed in Fig. 1 that these currents remain stable after repeated application of agonist during this same time frame. In an additional set of control experiments, we found that intracellular DIDS also blocks GABAAR-mediated currents (49 ± 7% within 20 min of whole cell recording, n = 4, data not shown) as previously reported (Albertson et al. 1996; Hollrigel et al. 1998). As expected, when postsynaptic GlyRs are blocked by DIDS, glycine application no longer was able to depress AMPAR currents elicited by exogenous glutamate application (Fig. 6B2). Moreover, inclusion of DIDS completely inhibited the glycine-induced depression of evoked EPSCs (Fig. 6, C and D; n = 7), and we observed no GlyR-mediated current and no change in Rin. Thus collectively, these findings provide strong evidence that a postsynaptic locus is the site of action of the GlyR-mediated depression of transmission.
|
) to minimize net movement of ions. In these experiments, it was necessary to examine subthreshold EPSPs (while blocking action potential generation with QX314 included in the pipette solution), because holding the membrane potential at the GlyR reversal potential is too near action potential threshold, and cells were randomly firing. Additionally, in these experiments, we were limited to an examination of only EPSPs because GABAergic inhibitory postsynaptic potentials (IPSPs) reverse at the same potential as GlyR-mediated currents. Thus, based on Ohms' Law, a synaptic current evoked when the membrane resistance is decreased (e.g., caused by open GlyR channels) will cause a smaller voltage change than when the resistance is higher (e.g., no open GlyR channels). Accordingly, it is predicted that the EPSP amplitude will be depressed by GlyR activation even if there is little to no net current through the open channels. In 5/10 recorded cells, the membrane potential was unchanged during glycine application but was slightly depolarized (1–3 mV) in the remaining 5 cells. Importantly, however, in all cells recorded, GlyR activation reversibly depressed the EPSP amplitude (Fig. 7; 31 ± 3% depression, n = 10) and the depression was blocked by 1 µM strychnine.
|
We were next interested in determining whether endogenously released glycine could modulate synaptic transmission through activation of GlyRs, similarly to what we have observed after exogenous glycine application. Electrical stimulation in CA1 s. radiatum releases glycine through a mechanism dependent on action potential generation, suggesting that at least some of the glycine released in hippocampus is of neural origin (Klancnik et al. 1992). Interestingly, blockade of GlyT1, the glycine transporter present in astrocytes (Zafra et al. 1995, 1997), potentiates evoked NMDAR-mediated currents in hippocampal slices (Bergeron et al. 1998) by elevating the extracellular glycine concentration in the vicinity of NMDARs. Here we tested whether preventing reuptake of glycine into astrocytes using the a potent GlyT1 transport inhibitor NFPS (Chen et al. 2003; Herdon et al. 2001) would cause accumulation of endogenously released glycine that could activate GlyRs and depress synaptically generated action potentials. In recordings from interneurons (n = 4), but not pyramidal cells (n = 4), we observed a depression of synaptically evoked suprathreshold EPSPs in the presence of low concentrations of NFPS (1 µM; Fig. 8). The NFPS-induced depression was antagonized by strychnine, indicating that the effect is mediated by GlyRs and not the result of a nonspecific action of the drug. As mentioned above, blocking GlyT1 with NPFS potentiates NMDAR currents in CA1 pyramidal cells (Bergeron et al. 1998), therefore we considered the possibility that the GlyR-mediated depression of EPSP amplitude was masked by an increase in NMDAR transmission. However, even when we included the NMDAR antagonist APV (100 µM) in the bath solution together with the NFPS, the EPSP amplitude still was not significantly depressed in pyramidal cells (5 ± 4% depression, n = 4, P > 0.05). It is unclear why the NFPS-induced depression of suprathreshold EPSPs was not observed in recordings from pyramidal cells similar to what was observed in interneurons, but this finding may indicate that GlyT1 on astrocytes are not expressed in the near vicinity of GlyRs on pyramidal cells. The GlyT2 transporter is expressed by neurons; however, pharmacological tools are not yet available commercially to test whether blocking this reuptake mechanism can modulate synaptic transmission recorded from pyramidal cells or interneurons. Nevertheless, these experiments using the GlyT1 antagonist clearly show that extracellular levels of endogenous glycine can be altered through modulation of glycine reuptake, suggesting that changes in the extracellular glycine concentration in vivo could lead to a depression of neuronal activity mediated through GlyR activation.
|
Inhibitory glycinergic interneurons in spinal cord and brain stem also contain and release GABA (Chery and de Koninck 1999; Jonas et al. 1998; O'Brien and Berger 1999). We therefore considered the possibility that the converse may be true in hippocampus, that GABAergic interneurons also contain glycine. We tested this idea using a highly specific anti-glycine antibody (Crook and Pow 1997; Pow et al. 1995) (generous gift of Dr. David Pow, University of Queensland) and found that hippocampal interneurons, but not pyramidal cells, are immunopositive for glycine (Fig. 9, A–D, G, and J). Additionally, presumed astrocytes were also observed to be glycine immunopositive (Fig. 9G, *), an expected result because previous studies have shown that these cells express the glycine transporter, GlyT1 (Zafra et al. 1995, 1997). In double-labeling experiments we find that all glycine-positive interneurons are also immunopositive for the neuronal glycine transporter GlyT2, a reliable marker for glycinergic neurons (Jursky and Nelson 1995; Zafra et al. 1995), which further supports the finding that these neurons are a source of glycine in hippocampus. Additionally, we show that interneurons, which are GABA and GAD immunopositive, are also glycine immunopositive (Fig. 9, G–L, arrows and arrowheads), indicating that hippocampal interneurons contain both inhibitory amino acids. Occasionally, we observed interneurons that are immunopositive for glycine only (Fig. 9, G–L). In glycine-GABA double-labeling studies, we found 14 cells immunopositive for glycine only and 87 cells immunopositive for both glycine and GABA (6 fields analyzed from 6 different sections). In glycine-GAD double labeling studies (5 fields analyzed from 5 different slices), of 209 cells counted, we found 11 glycine-only positive cells, with the remainder co-localizing glycine and GAD. These data suggest the interesting possibility that a subset of interneurons may use this inhibitory amino acid exclusively, although much more work is needed to confirm this initial observation. Together our immunohistochemical results support and extend the elegant studies of Danglot et al. (2004), where hippocampal interneurons were shown to express the glycine transporter, GlyT2.
|
|
|
DISCUSSION |
|---|
|
, 2003; Kirchner et al. 2003). Here, we extend our previous results (Chattipakorn and McMahon 2002) by showing that GlyR activation is capable of depressing activity in the hippocampal synaptic network. This ability of GlyRs could be the mechanism by which glycine and taurine, another GlyR agonist, depress seizure activity in some animal models of epilepsy, first reported two decades ago (Cherubini et al. 1981; Seiler and Sarhan 1984a, b). This is further supported in recent reports in hippocampal slices showing that GlyR activation can decrease hyperexcitibility in the dentate gyrus and area CA1 (Chattipakorn and McMahon 2003; Kirchner et al. 2003).
A major finding in our study is that GlyR activation depresses synaptically generated action potentials recorded from both pyramidal cells and interneurons, indicating that these receptors have a general function to limit activity in hippocampal circuits. In addition, we find in some cells strychnine increases excitability, indicating that GlyRs are tonically active and can set the ambient level of neuronal activity, as suggested by others (Mori et al. 2002), although it is worth mentioning that strychnine could have some nonspecific effects (Garcia-Colunga and Miledi 1999; Matsubayashi et al. 1998). Tonic inhibition is provided by extrasynaptic GABAARs (Farrant and Nusser 2005; Petrini et al. 2004), thus tonically active GlyRs are also likely to be extrasynaptic. This idea is supported by a recent anatomical study showing that nearly 70% of clustered GlyRs are not opposed by presynaptic terminals and are thus at extrasynaptic sites (Danglot et al. 2004).
GlyRs are expressed both pre- and postsynaptically in many brain regions; however, several findings suggest that the GlyRs responsible for depressing neuronal excitability and synaptic transmission are located at postsynaptic rather than at presynaptic sites. Clearly, depression of somatically induced action potentials through DC injection must be caused by a postsynaptic mechanism because synapses are not involved. The large decrease in Rin that accompanies GlyR activation is likely a major contributor to this depression of action potential generation because a given stimulus is much less effective in changing membrane voltage when the resistance is decreased by open channels. This mechanism could also easily explain the depression of synaptically induced action potentials (suprathreshold EPSPs). A postsynaptic mechanism is further supported by the larger depression of the EPSC amplitude when the postsynaptic GlyR current is increased by an increased driving force for chloride and also by the lack of depression of the EPSC amplitude when postsynaptic GlyRs are blocked by including DIDS in the pipette solution. However, a point that should be mentioned regarding the voltage-clamp experiments is that the magnitude of the postsynaptic GlyR current should, provided the recorded cells are well clamped, have no measurable effect on the amplitude of the EPSC, because the voltage-clamp circuit should compensate for the GlyR current that attempts to change membrane voltage. It is well-known that voltage control decreases with distance from the recording site (soma) (Carnevale et al. 1997; Spruston et al. 1993). Thus the larger synaptic depression, which accompanies the larger postsynaptic GlyR current, may be a consequence of inadequate space clamp. If true, this could indicate that the GlyRs responsible for the synaptic depression are "out of the reach" of the clamp, and may be in dendrites near the glutamatergic synapses, because somas are generally under good voltage control. Future studies involving direct recordings from dendrites will be needed to address this issue further. Finally, we cannot rule out some contribution of a GlyR mediated decrease in presynaptic release probability, even though we find no significant effect of GlyR activation on the PPF ratio (Dobrunz and Stevens 1997; Kim and Alger 2001; Zucker 1989).
Are GlyRs involved in fast inhibitory transmission in hippocampus? It seems possible because our immunohistochemical studies show that hippocampal interneurons co-contain glycine and GABA and also express the neuronal glycine transporter GlyT2 (Borowsky et al. 1993; Danglot et al. 2004). This suggests the interesting possibility that interneurons use both inhibitory neurotransmitters, similarly to interneurons in spinal cord and brain stem and Golgi cells in cerebellum which co-release glycine and GABA at mixed synapses (Chery and de Koninck 1999; Dumoulin et al. 2001; Jones 1993; O'Brien and Berger 1999). However, it seems that the majority of inhibitory synapses in hippocampus are devoid of GlyRs (Danglot et al. 2004; Levi et al. 2004; Meier and Grantyn 2004). Furthermore, data from electron microscopy studies show that when GlyRs are found at synapses, they are expressed at low density and are located near the edge of the postsynaptic density or just outside (Danglot et al. 2004). However, synaptic clustering of GlyRs can be increased when clustering of GABAARs is prevented by depletion of the gephyrin splice variant responsible for formation of GABAAR clusters (Meier and Grantyn 2004). This gephyrin isoform, but not the isoforms responsible for clustering GlyRs, is usually highly expressed at hippocampal synapses indicating a predominant synaptic localization of GABAARs and a most likely extrasynaptic location of GlyRs (Meier and Grantyn 2004). Taken together, these morphological data suggest that GlyRs may not be involved in fast synaptic inhibition in hippocampus. This potential synaptic GABAAR and extrasynaptic GlyR receptor distribution would thus explain why IPSCs at hippocampal synapses are blocked with GABAAR but not GlyR antagonists. Therefore the role of GlyRs in hippocampus may not be to mediate fast synaptic inhibition but instead to serve in a neuromodulatory role at extrasynaptic sites where they provide tonic inhibition, similarly to the tonic inhibition provided by extrasynaptic GABAARs (Farrant and Nusser 2005; Petrini et al. 2004). Thus functional data clearly supporting the notion that GlyRs mediate fast synaptic inhibition at hippocampal synapses awaits future confirmation.
Our data showing the depression of suprathreshold EPSPs (recorded from interneurons) after blockade of glycine reuptake into astrocytes (i.e., blockade of GlyT1) shows that endogenously released glycine can activate GlyRs and modulate neuronal excitability. The lack of an effect of GlyT1 blockade on evoked EPSPs recorded from pyramidal cells, similarly to that reported by Mori et al. (2002) in recordings from cultured hippocampal slices, could be caused by the co-localization of GlyT1 near glutamate synapses (Cubelos et al. 2005), which would regulate NMDAR activity, rather than being located near sites of GlyR expression on pyramidal cells. Because blockade of GlyT1 will prevent both glycine reuptake into astrocytes as well as glycine release that occurs after astrocyte depolarization, it seems that the source of the glycine that accumulates extracellularly in the presence of NFPS is not likely to be released from astrocytes and suggests that it may be of neural origin, likely from the interneurons through vesicular and/or transporter-mediated (GlyT2) release. Unfortunately development of pharmacological tools directed at GlyT2 lags behind that of GlyT1; therefore resolution of the functional role of GlyT2 awaits further clarification and investigation.
In summary, we propose that GlyRs participate in a novel inhibitory mechanism in hippocampus, modulating neuronal activity and synaptic transmission. The GlyR-mediated depression of synaptic potentials in hippocampus we report here is similar to the GlyR-mediated depression of nicotinic receptor–mediated EPSPs at synapses in the ciliary ganglia (Tsen et al. 2000), suggesting that this role of GlyRs in modulating synaptic efficacy could be a general mechanism applicable to many synapses throughout the autonomic and central nervous systems. Because inhibitory interneurons and excitatory pyramidal cells express GlyRs, we predict the net effect of GlyR activation in vivo is likely to be quite complex because selective activation of GlyRs on interneurons will cause disinhibition, whereas selective activation on pyramidal cells will cause net inhibition. Nevertheless, the findings in this study, together with our previously published work in dentate gyrus, show that globally enhancing GlyR activity throughout the network will cause net inhibition. Thus our findings indicate that therapeutic agents targeted at GlyRs, similarly to those that increase GABAA receptor activity, could be beneficial in depressing hyperexcitable hippocampal circuits that ensue in epilepsy, encouraging future studies into the precise location and function of these understudied inhibitory receptors.
|
|
GRANTS |
|---|
|
|
|
ACKNOWLEDGMENTS |
|---|
|
|
|
FOOTNOTES |
|---|
Address for reprint requests and other correspondence: L. L. McMahon, Dept. of Physiology and Biophysics, 1918 University Blvd., MCLM 964, Univ. of Alabama at Birmingham, Birmingham, AL 35294-0005 (E-mail: McMahon{at}physiology.uab.edu)
|
|
REFERENCES |
|---|
|
Baker AJ, Zornow MH, Scheller MS, Yaksh TL, Skilling SR, Smullin DH, Larson AA, and Kuczenski R. Changes in extracellular concentrations of glutamate, aspartate, glycine, dopamine, serotonin, and dopamine metabolites after transient global ischemia in the rabbit brain. J Neurochem 57: 1370–1379, 1991.[Web of Science][Medline]
Bergeron R, Meyer T, Coyle J, and Greene R. Modulation of N-methyl-D-aspartate receptor function by glycine transport. Proc Natl Sci USA 95: 15730–15734, 1998.
Borowsky B, Mezey E, and Hoffman BJ. Two glycine transporter variants with distinct localization in the CNS and peripheral tissues are encoded by a common gene. Neuron 10: 851–863, 1993.[CrossRef][Web of Science][Medline]
Carnevale NT, Tsai KY, Claiborne BJ, and Brown TH. Comparative electrotonic analysis of three classes of rat hippocampal neurons. J Neurophysiol 78: 703–720, 1997.
Chattipakorn SC and McMahon LL. Pharmacological characterization of glycine-gated chloride currents recorded in rat hippocampal slices. J Neurophysiol 87: 1515–1525, 2002.
Chattipakorn SC and McMahon LL. Strychnine-sensitive glycine receptors depress hyperexcitability in rat dentate gyrus. J Neurophysiol 89: 1339–1342, 2003.
Chen L, Muhlhauser M, and Yang CR. Glycine tranporter-1 blockade potentiates NMDA-mediated responses in rat prefrontal cortical neurons in vitro and in vivo. J Neurophysiol 89: 691–703, 2003.
Cherubini E, Bernardi G, Stanzione P, Marciani MG, and Mercuri N. The action of glycine on rat epileptic foci. Neurosci Lett 21: 93–97, 1981.[CrossRef][Web of Science][Medline]
Chery N and de Koninck Y. Junctional versus extrajunctional glycine and GABA(A) receptor-mediated IPSCs in identified lamina I neurons of the adult rat spinal cord. J Neurosci 19: 7342–7355, 1999.
Crook DK and Pow DV. Analysis of the distribution of glycine and GABA in amacrine cells of the developing rabbit retina: a comparison with the ontogeny of a functional GABA transport system in retinal neurons. Vis Neurosci 14: 751–763, 1997.[Web of Science][Medline]
Cubelos B, Gimenez C, and Zafra F. Localization of the GLYT1 glycine transporter at glutamatergic synapses in the rat brain. Cereb Cortex 15: 448–459, 2005.
Danglot L, Rostaing P, Triller A, and Bessis A. Morphologically identified glycinergic synapses in the hippocampus. Mol Cell Neurosci 27: 394–403, 2004.[CrossRef][Web of Science][Medline]
Deleuze C, Alonso G, Lefevre IA, Duvoid-Guillou A, and Hussy N. Extrasynaptic localization of glycine receptors in the rat supraoptic nucleus: further evidence for their involvement in glia-to-neuron communication. Neuroscience 133: 175–183, 2005.[CrossRef][Web of Science][Medline]
Deleuze C, Duvoid A, and Hussy N. Properties and glial origin of osmotic-dependent release of taurine from the rat supraoptic nucleus. J Physiol 507: 463–471, 1998.
Dobrunz LE and Stevens CF. Heterogeneity of release probability, facilitation, and depletion at central synapses. Neuron 18: 995–1008, 1997.[CrossRef][Web of Science][Medline]
Dugue GP, Dumoulin A, Triller A, and Dieudonne S. Target-dependent use of coreleased inhibitory transmitters at central synapses. J Neurosci 25: 6490–6498, 2005.
Dumoulin A, Triller A, and Dieudonne S. IPSC kinetics at identified GABAergic and mixed GABAergic and glycinergic synapses onto cerebellar Golgi cells. J Neurosci 21: 6045–6057, 2001.
Farrant M and Nusser Z. Variations on an inhibitory theme: phasic and tonic activation of GABA(A) receptors. Nat Rev Neurosci 6: 215–229, 2005.[CrossRef][Web of Science][Medline]
Flint AC, Liu X, and Kriegstein AR. Nonsynaptic glycine receptor activation during early neocortical development. Neuron 20: 43–53, 1998.[CrossRef][Web of Science][Medline]
Garcia-Colunga J and Miledi R. Modulation of nicotinic acetylcholine receptors by strychnine. Proc Natl Sci USA 96: 4113–4118, 1999.
Ghavanini AA, Mathers DA, and Puil E. Glycinergic inhibition in thalamus revealed by synaptic receptor blockade. Neuropharmacology 49: 338–349, 2005.[CrossRef][Web of Science][Medline]
Herdon HJ, Godfrey FM, Brown AM, Coulton S, Evans JR, and Cairns WJ. Pharmacological assessment of the role of the glycine transporter GlyT-1 in mediating high-affinity glycine uptake by rat cerebral cortex and cerebellum synaptosomes. Neuropharmacology 41: 88–96, 2001.[CrossRef][Web of Science][Medline]
Hollrigel GS, Ross ST, and Soltesz I. Temporal patterns and depolarizing actions of spontaneous GABAA receptor activation in granule cells of the early postnatal dentate gyrus. J Neurophysiol 80: 2340–2351, 1998.
Hussy N, Bres V, Rochette M, Duvoid A, Alonso G, Dayanithi G, and Moos FC. Osmoregulation of vasopressin secretion via activation of neurohypophysial nerve terminals glycine receptors by glial taurine. J Neurosci 21: 7110–7116, 2001.
Ito S and Cherubini E. Strychnine-sensitive glycine responses of neonatal rat hippocampal neurones. J Physiol 440: 67–83, 1991.
Jackson MF, Esplin B, and Capek R. Inhibitory nature of tiagabine-augmented GABAA receptor-mediated depolarizing responses in hippocampal pyramidal cells. J Neurophysiol 81: 1192–1198, 1999.
Jonas P, Bischofberger J, and Sandkuhler J. Corelease of two fast neurotransmitters at a central synapse. Science 281: 419–424, 1998.
Jones EG. GABAergic neurons and their role in cortical plasticity in primates. Cereb Cortex 3: 361–372, 1993.
Jursky F and Nelson N. Localization of glycine neurotransmitter transporter (GLYT2) reveals correlation with the distribution of glycine receptor. J Neurochem 64: 1026–1033, 1995.[Web of Science][Medline]
Karkar KM, Thio LL, and Yamada KA. Effects of seven clinically important antiepileptic drugs on inhibitory glycine receptor currents in hippocampal neurons. Epilepsy Res 58: 27–35, 2004.[CrossRef][Web of Science][Medline]
Kawa K. Glycine receptors and glycinergic synaptic transmission in the deep cerebellar nuclei of the rat: a patch-clamp study. J Neurophysiol 90: 3490–3500, 2003.
Kim J and Alger BE. Random response fluctuations lead to spurious paired-pulse facilitation. J Neurosci 21: 9608–9618, 2001.
Kirchner A, Breustedt J, Rosche B, Heinemann UF, and Schmieden V. Effects of taurine and glycine on epileptiform activity induced by removal of mg2+ in combined rat entorhinal cortex-hippocampal slices. Epilepsia 44: 1145–1152, 2003.[CrossRef][Web of Science][Medline]
Klancnik JM, Cuenod M, Gahwiler BH, Jiang ZP, and Do KQ. Release of endogenous amino acids, including homocysteic acid and cysteine sulphinic acid, from rat hippocampal slices evoked by electrical stimulation of Schaffer collateral-commissural fibres. Neuroscience 49: 557–570, 1992.[CrossRef][Web of Science][Medline]
Leewanich P, Tohda M, Matsumoto K, Subhadhirasakul S, Takayama H, Aimi N, and Watanabe H. A possible mechanism underlying corymine inhibition of glycine-induced Cl- current in Xenopus oocytes. Eur J Pharmacol 348: 271–277, 1998.[CrossRef][Web of Science][Medline]
Levi S, Logan SM, Tovar KR, and Craig AM. Gephyrin is critical for glycine receptor clustering but not for the formation of functional GABAergic synapses in hippocampal neurons. J Neurosci 24: 207–217, 2004.
Maccaferri G and McBain CJ. Long-term potentiation in distinct subtypes of hippocampal nonpyramidal neurons. J Neurosci 16: 5334–5343, 1996.
Malosio ML, Marqueze-Pouey B, Kuhse J, and Betz H. Widespread expression of glycine receptor subunit mRNAs in the adult and developing rat brain. EMBO J 10: 2401–2409, 1991.[Web of Science][Medline]
Mangin JM, Guyon A, Eugene D, Paupardin-Tritsch D, and Legendre P. Functional glycine receptor maturation in the absence of glycinergic input in dopaminergic neurones of the rat substantia nigra. J Physiol 542: 685–697, 2002.
Matsubayashi H, Alkondon M, Pereira EF, Swanson KL, and Albuquerque EX. Strychnine: a potent competitive antagonist of alpha-bungarotoxin-sensitive nicotinic acetylcholine receptors in rat hippocampal neurons. J Pharmacol Exp Ther 284: 904–913, 1998.
McCool BA. Subunit composition of strychnine-sensitive glycine receptors expressed by adult rat basolateral amygdala neurons. Eur J Neurosci 14: 1082–1090, 2001.[CrossRef][Web of Science][Medline]
McMahon LL and Kauer JA. Hippocampal interneurons express a novel form of synaptic plasticity. Neuron 18: 295–305, 1997.[CrossRef][Web of Science][Medline]
Meier J and Grantyn R. A gephyrin-related mechanism restraining glycine receptor anchoring at GABAergic synapses. J Neurosci 24: 1398–1405, 2004.
Mody I. Ion channels in epilepsy. Int Rev Neurobiol 42: 199–226, 1998.[Web of Science][Medline]
Mori M, Gahwiler BH, and Gerber U. Beta-alanine and taurine as endogenous agonists at glycine receptors in rat hippocampus in vitro. J Physiol 539: 191–200, 2002.
O'Brien JA and Berger AJ. Cotransmission of GABA and glycine to brain stem motoneurons. J Neurophysiol 82: 1638–1641, 1999.
Petrini EM, Marchionni I, Zacchi P, Sieghart W, and Cherubini E. Clustering of extrasynaptic GABA(A) receptors modulates tonic inhibition in cultured hippocampal neurons. J Biol Chem 279: 45833–45843, 2004.
Pow DV, Wright LL, and Vaney DI. The immunocytochemical detection of amino-acid neurotransmitters in paraformaldehyde-fixed tissues. J Neurosci Methods 56: 115–123, 1995.[CrossRef][Web of Science][Medline]
Saransaari P and Oja SS. Enhanced taurine release in cell-damaging conditions in the developing and ageing mouse hippocampus. Neuroscience 79: 847–854, 1997.[CrossRef][Web of Science][Medline]
Saransaari P and Oja SS. Mechanisms of ischemia-induced taurine release in mouse hippocampal slices. Brain Res 807: 118–124, 1998.[CrossRef][Web of Science][Medline]
Saransaari P and Oja SS. Characteristics of ischemia-induced taurine release in the developing mouse hippocampus. Neuroscience 94: 949–954, 1999.[CrossRef][Web of Science][Medline]
Scharfman HE and Schwartzkroin PA. Responses of cells of the rat fascia dentata to prolonged stimulation of the perforant path: sensitivity of hilar cells and changes in granule cell excitability. Neuroscience 35: 491–504, 1990.[CrossRef][Web of Science][Medline]
Seiler N and Sarhan S. Synergistic anticonvulsant effects of GABA-T inhibitors and glycine. Naunyn Schmiedebergs Arch Pharmacol 326: 49–57, 1984a.[CrossRef][Web of Science][Medline]
Seiler N and Sarhan S. Synergistic anticonvulsant effects of a GABA agonist and glycine. Gen Pharmacol 15: 367–369, 1984b.[Web of Science][Medline]
Sergeeva OA and Haas HL. Expression and function of glycine receptors in striatal cholinergic interneurons from rat and mouse. Neuroscience 104: 1043–1055, 2001.[CrossRef][Web of Science][Medline]
Sloviter RS. Decreased hippocampal inhibition and a selective loss of interneurons in experimental epilepsy. Science 235: 73–76, 1987.
Spruston N, Jaffe DB, Williams SH, and Johnston D. Voltage- and space-clamp errors associated with the measurement of electrotonically remote synaptic events. J Neurophysiol 70: 781–802, 1993.
Staley KJ and Mody I. Shunting of excitatory input to dentate gyrus granule cells by a depolarizing GABAA receptor-mediated postsynaptic conductance. J Neurophysiol 68: 197–212, 1992.
Sun HY, Lyons SA, and Dobrunz LE. Mechanisms of target-cell specific short-term plasticity at Schaffer collateral synapses onto interneurons vs. pyramidal cells in juvenile rats. J Physiol 568: 815–840, 2005.
Tsen G, Williams B, Allaire P, Zhou Y-D, Ikonomov O, Knodova I, and Jacob M. Receptors with opposing functions are in postsynaptic microdomains under one presynaptic terminal. Nat Neurosci 3: 126–132, 2000.[CrossRef][Web of Science][Medline]
Turecek R and Trussell LO. Presynaptic glycine receptors enhance transmitter release at a mammalian central synapse. Nature 411: 587–590, 2001.[CrossRef][Medline]
Wang F, Xiao C, and Ye JH. Taurine activates excitatory non-synaptic glycine receptors on dopamine neurones in ventral tegmental area of young rats. J Physiol 565: 503–516, 2005.
Wang P and Slaughter MM. Effects of GABA receptor antagonists on retinal glycine receptors and on homomeric glycine receptor alpha subunits. J Neurophysiol 93: 3120–3126, 2005.
Wilcox KS, Fitzsimonds RM, Johnson B, and Dichter MA. Glycine regulation of synaptic NMDA receptors in hippocampal neurons. J Neurophysiol 76: 3415–3424, 1996.
Xu H, Zhou KQ, Huang YN, Chen L, and Xu TL. Taurine activates strychnine-sensitive glycine receptors in neurons of the rat inferior colliculus. Brain Res 1021: 232–240, 2004.[CrossRef][Web of Science][Medline]
Ye G, Tse AC, and Yung W. Taurine inhibits rat substantia nigra pars reticulata neurons by activation of GABA- and glycine-linked chloride conductance. Brain Res 749: 175–179, 1997.[CrossRef][Web of Science][Medline]
Ye JH, Schaefer R, Wu WH, Liu PL, Zbuzek VK, and McArdle JJ. Inhibitory effect of ondansetron on glycine response of dissociated rat hippocampal neurons. J Pharmacol Exp Ther 290: 104–111, 1999.
Ye JH, Tao L, Ren J, Schaefer R, Krnjevic K, Liu PL, Schiller DA, and McArdle JJ. Ethanol potentiation of glycine-induced responses in dissociated neurons of rat ventral tegmental area. J Pharmacol Exp Ther 296: 77–83, 2001.
Ye JH, Wang F, Krnjevic K, Wang W, Xiong ZG, and Zhang J. Presynaptic glycine receptors on GABAergic terminals facilitate discharge of dopaminergic neurons in ventral tegmental area. J Neurosci 24: 8961–8974, 2004.
Zafra F, Aragon C, Olivares L, Danbolt NC, Gimenez C, and Storm-Mathisen J. Glycine transporters are differentially expressed among CNS cells. J Neurosci 15: 3952–3969, 1995.[Abstract]
Zafra F, Poyatos I, and Gimenez C. Neuronal dependency of the glycine transporter GLYT1 expression in glial cells. Glia 20: 155–162, 1997.[CrossRef][Web of Science][Medline]
Zhao D and Leung LS. Effects of hippocampal kindling on paired-pulse response in CA1 in vitro. Brain Res 564: 220–229, 1991.[CrossRef][Web of Science][Medline]
Zhao P, Qian H, and Xia Y. GABA and glycine are protective to mature but toxic to immature rat cortical neurons under hypoxia. Eur J Neurosci 22: 289–300, 2005.[CrossRef][Web of Science][Medline]
Zucker RS. Short-term synaptic plasticity. Annu Rev Neurosci 12: 13–31, 1989.[CrossRef][Web of Science][Medline]
This article has been cited by other articles:
|
|
 |
|
  T. Keck, K. P. Lillis, Y.-D. Zhou, and J. A. White Frequency-Dependent Glycinergic Inhibition Modulates Plasticity in Hippocampus J. Neurosci., July 16, 2008; 28(29): 7359 - 7369. [Abstract] [Full Text] [PDF]
|
|
|
|
 |
|
 X.-B. Zhang, G.-C. Sun, L.-Y. Liu, F. Yu, and T.-L. Xu {alpha}2 Subunit Specificity of Cyclothiazide Inhibition on Glycine Receptors Mol. Pharmacol., April 1, 2008; 73(4): 1195 - 1202. [Abstract] [Full Text] [PDF]
|
|
|
|
 |
|
 H. X. Zhang and L. L. Thio Zinc Enhances the Inhibitory Effects of Strychnine-Sensitive Glycine Receptors in Mouse Hippocampal Neurons J Neurophysiol, December 1, 2007; 98(6): 3666 - 3676. [Abstract] [Full Text] [PDF]
|
|
|
|
 |
|
 I. Marchionni, A. Omrani, and E. Cherubini In the developing rat hippocampus a tonic GABAA-mediated conductance selectively enhances the glutamatergic drive of principal cells J. Physiol., June 1, 2007; 581(2): 515 - 528. [Abstract] [Full Text] [PDF]
|
|
|
|
 |
|
 Highlights From The Literature Physiology, April 1, 2006; 21(2): 83 - 85. [Full Text] [PDF]
|
|
| ||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||||
| HOME | HELP | FEEDBACK | SUBSCRIPTIONS | ARCHIVE | SEARCH | TABLE OF CONTENTS |
| Visit Other APS Journals Online |
TOP
ABSTRACT
INTRODUCTION
, n = 5) and interneurons (
, n = 7). All cells were recorded with CsCl pipette solution (ECl– = 0 mV) and holding potential was –70 mV.
) to block potential glycine-mediated increase in NMDAR currents. The percentage of trials generating suprathreshold EPSPs in pyramidal cells during glycine application was decreased by 22 ± 8% in the absence of NMDAR blockade (n = 4) and by 32 ± 6% when NMDARs were blocked by D-APV (n = 6, P > 0.08 in the absence vs. presence of D-APV). In interneurons, percentage of trials generating suprathreshold EPSPs was decreased by 27 ± 8% (n = 4) in the absence and 33 ± 5% in the presence of NMDAR blockade with D-APV (100 µM; n = 6, P > 0.25 in the absence vs. presence of D-APV). Magnitude of depression observed in pyramidal cells is not significantly different from that in interneurons (P > 0.05). All cells were recorded with K+ gluconate pipette solution and were held at their resting membrane potential (pyramidal cells: 67 ± 1 mV, n = 10; interneurons: 68 ± 1 mV, n = 10).
