ARTICLE

Distinct Subtypes of Metabotropic Glutamate Receptors Mediate Differential Actions on Excitability of Spinal Respiratory Motoneurons

Xiao-Wei Dong and Jack L. Feldman
Journal of Neuroscience 1 July 1999, 19 (13) 5173-5184; https://doi.org/10.1523/JNEUROSCI.19-13-05173.1999

Abstract

Metabotropic glutamate receptors (mGluRs) modulate neuronal function by affecting excitability and altering synaptic transmission. We have shown that the mGluR agonist (1S,3R)-1-amino-1,3-cyclopentanedicarboxylic acid (1S,3R-ACPD) has multiple actions on phrenic motoneurons (PMNs), including reduction of inspiratory-modulated synaptic currents and an increase of neuronal excitability. We hypothesized that these actions were mediated by different mGluR subtypes. We have now identified the involvement of mGluR subtypes and their roles in modulating the excitability of PMNs and the consequent inspiratory motor output in an in vitro neonatal rat brainstem–spinal cord preparation. Activation of postsynaptic group-I mGluRs increases PMN excitability, associated with the production of an inward current and a decrease in membrane conductance, whereas activation of group-II or group-III mGluRs decreases PMN inspiratory-modulated synaptic current, probably via a presynaptic mechanism. To confirm further the distinction and the involvement of group-I and group-II/-III receptor subtypes affecting PMN excitability, we used the membrane permeable cAMP analog 8-bromo-cAMP (8-Br-cAMP) to elevate intracellular cAMP concentration to mask or occlude any effects mediated via the cAMP cascade. 8-Br-cAMP attenuated the reduction of the inspiratory-modulated activity of PMNs by both (S)-4-carboxy-3-hydroxyphenylglycine (4C3HPG) andl-(+)-2-amino-4-phosphonobutyric acid (l-AP4), agonists for group-II and group-III mGluRs, respectively, but did not affect the actions of 3,5-dihydroxyphenylglycine (DHPG), an agonist for group-I mGluRs. These three groups of mGluRs are all endogenously activated during the inspiratory phase. We conclude that three groups of mGluRs are functionally expressed in the phrenic nucleus and that their activation modulates PMN excitability via distinct mechanisms, with group-I acting at postsynaptic sites and group-II and group-III acting at presynaptic sites.

Metabotropic glutamate receptors (mGluRs) modulate neuronal function via affecting excitability and altering synaptic transmission (Schoepp and Conn, 1993; Gallagher et al., 1994; Pin and Duvoisin, 1995). The diversity of mGluR actions can be primarily attributed to different receptor subtypes [mGluR1–8 (Pin and Bockaert, 1995)] and their cellular localizations. Group-I mGluRs (mGluR1 and mGluR5) are coupled to phospholipase C and increase the synthesis of inositol 1,4,5-trisphosphate (Masu et al., 1991; Abe et al., 1992; Aramori and Nakanishi, 1992); they can be selectively activated by 3,5-dihydroxyphenylglycine (DHPG) (Schoepp et al., 1994). Group-I mGluRs appear to be localized postsynaptically (Martin et al., 1992; Baude et al., 1993; Lujan et al., 1996; Shigemoto et al., 1997) where they act to increase neuronal excitability (Davies et al., 1995;Netzeband et al., 1997; Schoppa and Westbrook, 1997; Schrader and Tasker, 1997). Group-II (mGluR2 and mGluR3) and group-III (mGluR4 and mGluR6–8) mGluRs are negatively coupled to adenylyl cyclase and inhibit the formation of cAMP (Tanabe et al., 1992, 1993; Nakajima et al., 1993; Okamoto et al., 1994; Saugstad et al., 1994; Duvoisin et al., 1995). Group-II and group-III receptors are predominantly localized in presynaptic terminals (Shigemoto et al., 1995, 1996, 1997) where they inhibit transmitter release (Forsythe and Clements, 1990;Baskys and Malenka, 1991; Trombley and Westbrook, 1992; Gereau and Conn, 1995; Salt and Eaton, 1995; Vignes et al., 1995; Macek et al., 1996; Schrader and Tasker, 1997).

The physiological roles of mGluR subtypes in identified neurons with measurable behaviors warrant investigation. Although the effects of different mGluRs in single neurons have been extensively reported (Poncer et al., 1995; Salt and Eaton, 1995; Macek et al., 1996; Libri et al., 1997; Schoppa and Westbrook, 1997; Schrader and Tasker, 1997), their roles in regulating integrative functions or in behavior are poorly understood. In this study, we examine the actions of different mGluRs affecting respiratory motor output, in particular, on phrenic motoneurons (PMNs) that receive inspiratory drive from the brainstem and control the diaphragm, the principal inspiratory muscle. We performed this study in an in vitro brainstem–spinal cord preparation, in which the transmission of endogenous inspiratory drive to PMNs is mediated by glutamate acting primarily at non-NMDA receptors (McCrimmon et al., 1989; Liu et al., 1990; Feldman and Smith, 1994). Thus, we can study mGluR actions at an identified, endogenously driven glutamatergic synapse onto a functionally identified neuron participating in a meaningful and measurable behavior. A broad spectrum mGluR agonist (1S,3R)-1-amino-1,3-cyclopentanedicarboxylic acid (1S,3R-ACPD) reduces inspiratory-modulated synaptic currents and increases the excitability of PMNs (Dong et al., 1996). These actions are mediated by distinct mechanisms at pre- and postsynaptic sites. We have now identified the mGluR subtypes underlying these effects by examining the actions of specific agonists on endogenous inspiratory-modulated synaptic current, baseline membrane current, and action potential patterns in PMNs. We then examined the effects of perturbing second messenger pathways associated with group-I and group-II/-III receptor subtypes. We analyzed the effects of these various perturbations on postsynaptic membrane properties of PMNs and on the frequency and amplitude of miniature EPSCs (mEPSCs).

Parts of this paper have been published previously (Dong and Feldman, 1995b, 1996).

MATERIALS AND METHODS

En bloc preparation. Experiments were performed onin vitro preparations of brainstem and spinal cord from 0- to 4-d-old neonatal rats. Details of the preparation have been described elsewhere (Smith and Feldman, 1987; Liu et al., 1990; Dong and Feldman, 1995a). In brief, the brainstem and cervical spinal cord were isolated from 0- to 4-d-old Sprague Dawley rats anesthetized with ether or hypothermia. The en bloc neuraxis was then pinned down with the ventral surface upward on Sylgard resin in a recording chamber and continuously superfused with normal artificial CSF (aCSF) (in mm): 128 NaCl, 3 KCl, 1.5 CaCl2, 1 MgSO4, 21 NaHCO3, 0.5 NaH2PO4, and 30 d-glucose, equilibrated with 95% O2/5% CO2. The bath temperature was gradually raised from 10–15°C (for isolation) to 25–26°C before recording.

Electrophysiology. Respiratory activity was recorded with suction electrodes from the C4 ventral root, which contains phrenic motoneuronal axons, and sometimes simultaneously from cranial nerves (X and XII). Signals were amplified (Grass P511K; Grass Instrument, Quincy, MA), rectified, and low-pass filtered (Paynter filter; τ = 15 msec).

Electrodes for whole-cell patch-clamp recordings were pulled from aluminosilicate glass (A-M Systems, Everett, WA) with a tip size of ∼2 μm and a resistance of 3.5–5 MΩ when filled with solution containing (in mm): 120 K+-gluconate, 1 CaCl2, 5 NaCl, 10 HEPES, 2 ATP (magnesium salt), and 10 1,2-bis-(2-aminophenoxy)ethane-N,N,N′,N′-tetra-acetic acid (tetrapotassium salt), at pH 7.3 adjusted by KOH. Successful whole-cell recording was ensured by the initial formation of a gigaohm seal (2–10 GΩ) and low series resistance (RS ; 8–15 MΩ). RS was estimated using 100 Hz, −10 mV, 5 msec voltage pulses. When in voltage-clamp mode, a 60–80%RS compensation was used. During experiments, RS was frequently checked, and data were discarded if large increases occurred during the course of the recording. PMNs were voltage-clamped at the end-expiratory potentials of −60 to −75 mV. Data obtained from PMNs displaying fast Na+ currents during inspiration (indicative of poor space clamp) were not included in the analysis. Signals were amplified with a patch-clamp amplifier (AXOPATCH 1D or AXOPATCH 200; Axon Instruments, Foster City, CA) and filtered at 2–5 kHz (Bessel filter).

Current–voltage (I–V) relations were obtained by applying a series of command voltage step pulses (step size, 2–5 mV; width, 100–200 msec; frequency, 2 Hz) controlled by software (Axodata or Axoscope; Axon Instruments). I–V curves were obtained by plotting current change (averaged steady-state current values at 5–10 msec before offset of voltage step) against membrane potential. Because most PMNs did not exhibit slow time-dependent membrane properties over the testing voltage range and the membrane current reached steady state at 50 msec after the onset of a voltage pulse (Dong et al., 1996), steady-state current could be obtained using voltage pulses with widths ≥100 msec. Membrane potentials (Vm) were adjusted for liquid junction potentials (−10 mV). Neuron input conductance (GN ) was calculated at the holding potential (−60 to −75 mV) from the slope of a least-squares regression line fitted to the data.

Neurons subjected to experimental measurements and data analysis satisfied various criteria described previously (Liu et al., 1990;Lindsay and Feldman, 1993). Briefly, these neurons had resting membrane potentials of at least −60 mV and displayed rhythmic synaptic drive currents in synchrony with the inspiratory burst activity on the C4 ventral root. These neurons were located at intermediate laterality and 130–300 μm below the ventral surface at the C4 segment, consistent with the location of the PMN pool in neonatal rats (Lindsay et al., 1991). Axons of these neurons were contained in the C4 ventral root, indicated by antidromic activation by stimulating the C4 nerve through the suction electrode. Moreover, their other intrinsic properties, such as input resistance, were consistent with the measurements made in neurons identified as PMNs (Smith et al., 1988).

Pharmacological substances and application. The drugs used included (RS)-DHPG (Tocris Cookson, Ballwin, MO; 30–200 μm), (S)-4-carboxy-3-hydroxyphenylglycine (4C3HPG; Tocris Cookson; 30–500 μm),l-(+)-2-amino-4-phosphonobutyric acid (l-AP4; Tocris Cookson; 3–50 μm), (RS)-1-aminoindan-1,5-dicarboxylic acid (AIDCA; Tocris Cookson; 2 mm), (2S)-α-ethylglutamic acid (EGLU; Tocris Cookson; 2 mm), (RS)-α-methylserine-O-phosphate (MSOP; Tocris Cookson; 1–2 mm), 8-bromo-cAMP (8-Br-cAMP; Research Biochemicals, Natick, MA; 0.8–1.2 mm), 6-cyano-7-nitroquinoxaline-2,3-dione (CNQX; Tocris Cookson; 100 μm), (+)-5-methyl-10,11-dihydro-5H-dibenzo [a,d] cyclohepten-5,10-iminemaleate (MK-801; Research Biochemicals; 250 μm), and tetrodotoxin (TTX; Sigma, St. Louis, MO; 1 μm).

Experiments were performed while preparations were perfused with normal aCSF solution as described above. Drugs were added to the spinal cord bath and/or applied locally via a glass pipette placed over the midcervical spinal cord region containing the PMN pool. Bath application was used to determine the minimum concentrations required for drug action. With bath application of drugs, the chamber was partitioned into two compartments at the level of the spinomedullary junction by a transverse barrier of petroleum jelly (Vaseline) across the neuraxis (Liu et al., 1990). This allows selective drug application to the spinal cord to affect synaptic transmission at the spinal level without disturbing processes at the brainstem level, where the descending inspiratory motor drive originates. Drugs were added to the spinal compartment at concentrations starting from the minimum necessary to induce a clear change in C4 root activity, and 6–8 min was allowed for equilibrium.

Vaseline often caused difficulty in obtaining good seals for patch recording. Thus, when such recordings were desired, test agents were applied locally in an unpartitioned chamber via pressure ejection from single- or multibarrel pipettes positioned close to the ventral surface of the midcervical spinal cord over the PMN pool (Liu et al., 1990). Each barrel had an orifice of 8–10 μm and was filled with a drug solution, saline, or aCSF. Application of drugs was controlled by brief air pressure pulses to the appropriate drug barrel. Control injections were made by ejecting saline or aCSF. The observed change caused by a test drug acting at a spinal site rather than at a supraspinal site was indicated by unchanged respiratory rate recorded from the C4 root and unchanged amplitude recorded from cranial nerves (X and XII).

In experiments examining the effect of changing intracellular cAMP concentration on drug action with C4 root recording, bath application of 8-Br-cAMP was combined with local application of an agonist. Thus, after the effect of a locally applied agonist was examined, 8-Br-cAMP was added to the spinal compartment, and then the agonist was tested again. The application of 8-Br-cAMP began at least 8–10 min before agonist application and continued during the agonist test.

Data acquisition and analysis. Data were recorded on videotape via pulse code modulation (Vetter model 3000; A. R. Vetter, Rebersburg, PA; sampled at 10–40 kHz per channel) for off-line analysis. Selected segments of records were digitized at 5–25 kHz using an analog-to-digital converter and were stored on a Vaxstation 3200 computer disk (Digital Equipment Corporation, Maynard, MA) or on a Pentium computer disk for subsequent computer-aided analysis.

For analysis of changes of respiratory drive, the average values of peak amplitude and area of inspiratory-modulated synaptic current (charge transfer) or integrated C4 ventral root discharges were computed from respiratory cycles before and after drug application. Statistical values are reported as means ± SEM. Differences between means were assessed by Student’s t test, and a value of p < 0.05 was considered significant.

For analysis of perturbations of frequency and amplitude of mEPSCs, the data were first filtered using a Wiener (optimal) filter (Press et al., 1989; Barkat, 1991), which greatly attenuates background noise without significantly affecting the characteristics of the original signal (Liu and Feldman, 1992). Events were detected using a threshold detector. Then under visual inspection, events above noise level were collected for data analysis. The reliability of detection of unitary events was ensured by a high signal-to-noise ratio (>2.2) (Liu and Feldman, 1992); the amplitudes of mEPSCs were well above noise level in each cell tested. We did not observe any presumptive mEPSCs of size below 2.2 × the mean noise level. We therefore assume that we detected almost all spontaneous EPSCs. To ensure identical voltage control before and after drug treatment so that the error in amplitude measurement because of inadequate space clamp would be similar under these two conditions, we monitored the series resistance and discarded data if significant increases occurred during the course of the recording. All collected EPSCs were then subject to analysis. For each condition, cumulative probability distribution histograms for interval and amplitude were constructed. Statistical significance for the difference between distributions was assessed by the Kolmogorov–Smirnov test (Van der Kloot, 1991), and a value ofp < 0.05 was considered significant.

RESULTS

Phrenic motoneurons receive rhythmic excitatory inspiratory inputs from bulbospinal inspiratory neurons. Under voltage-clamp conditions in the brainstem–spinal cord preparation, PMNs exhibit large, fast-rising, and slow-declining EPSCs during the inspiratory phase of the respiratory cycle (Fig. 1) (Liu et al., 1990; Dong et al., 1996). C4 ventral roots, which contain PMN axons, display spontaneous periodic bursts of discharges representing PMN population activity during the inspiratory phase (Fig. 1).

Fig. 1.
Fig. 1.

Effects of the group-I mGluR agonist DHPG on membrane currents of a PMN and the activity in C4 ventral roots.A, Raw traces of simultaneously recorded C4 ventral root activity (C4; top) and membrane current (Im ; bottom) of a PMN showing responses to locally applied DHPG (200 μm; period of DHPG application indicated by the horizontal line). At this concentration, DHPG caused tonic activity in C4 roots. Concurrently, DHPG induced an inward current in the PMN, which was voltage-clamped at the end-expiratory potential (Vh) of −64 mV. Note that the inspiratory drive current was not significantly affected. B, Superimposed inspiratory drive currents (Im ) and integrated C4 root activity (∫C4) before and during the treatment with a lower concentration (100 μm, local) of DHPG. Inspiratory drive currents were not significantly affected by DHPG. The inspiratory discharges of C4 roots were increased.Traces are averages from six consecutive inspiratory phases in control conditions and during the period of peak effect on C4 activity after drug application. C, Summary of effects of DHPG (100 μm, local) on peak inspiratory drive currents and C4 discharges. Vertical bars are averages from six successive inspiratory phases of peak inspiratory drive currents (left) and integrated inspiratory discharges of C4 (∫C4; right) during peak effect of the drug pooled from eight and six preparations, respectively. Error bars indicate SEM. An asterisk indicates a significant difference (p < 0.05; ttest) from control values. Insp, Inspiratory.D, Raw trace showing the persistence of DHPG-induced inward current in a PMN after the bath application of a cocktail containing TTX (1 μm) and ionotropic glutamate receptor antagonists CNQX (100 μm) and MK-801 (250 μm).

Enhancement of excitability of PMNs by group-I mGluRs

To determine the role of group-I mGluRs in affecting PMN excitability, we examined the effect of an agonist for group-I mGluRs, DHPG (Schoepp et al., 1994), on membrane currents of PMNs and on C4 ventral root activity. DHPG (50–200 μm, local) produced an inward current (IDHPG; 50–200 pA) in all PMNs examined (n = 8) when the membrane potentials were clamped at end-expiratory potentials (−60 to −75 mV; Fig. 1). The inspiratory-modulated synaptic currents, however, were not significantly affected (96 ± 6%; n = 8; Fig. 1A–C). Inspiratory discharges in C4 ventral roots increased at low concentrations of DHPG (≤150 μm, local; n = 12; Fig.1B,C). At 100 μm DHPG (local), the integrated C4 root discharge increased to 123 ± 8% of control (n = 6; Fig. 1C). At high concentrations (>150 μm, local), DHPG induced tonic discharges in the C4 roots (n = 6; Fig.1A). No changes in respiratory frequency (Fig.1A) or in inspiratory activity of cranial nerves (X and XII) (data not shown) were observed after local application of DHPG to the midcervical spinal cord.

The current induced by DHPG could result from actions of DHPG in addition to its presumed effect on postsynaptic group-I mGluRs, including (1) increased activity of spinal interneurons projecting to PMNs and (2) actions mediated by ionotropic GluRs. To elucidate the mechanisms underlying IDHPG, we examined the effects of DHPG after treatment with TTX (1 μm) to block voltage-dependent Na+ action potentials and associated synaptic transmission and with MK-801 (250 μm) and CNQX (100 μm), NMDA and non-NMDA receptor antagonists, respectively, to block currents mediated by ionotropic glutamate receptors. Under these conditions, DHPG continued to produce inward currents (six of six neurons; Fig. 1D), indicating a direct action on postsynaptic mGluRs of PMNs.

Suppression of synaptic transmission to PMNs by group-II and group-III

We showed previously (Dong et al., 1996) that simultaneous activation of different mGluR subtypes by 1S,3R-ACPD, a broad-spectrum agonist, affected several currents in PMNs, including the induction of an inward current and the decrease of inspiratory drive current. Because the above results indicate that group-I mGluRs induce an inward current but do not affect inspiratory drive current, receptors in other groups were candidates for mediating the suppression of inspiratory drive current. We therefore examined the role of group-II mGluRs by testing the effect of an agonist, 4C3HPG (Birse et al., 1993; Kingston et al., 1995), on PMN membrane currents and C4 ventral root activity. 4C3HPG decreased inspiratory drive current and spontaneous EPSCs during the expiratory phase (n = 7), with no detectable effects on baseline membrane current (Fig.2B). The reductions of peak and total charge transfer of inspiratory drive current by locally applied 4C3HPG (500 μm) were 53 ± 8 and 58 ± 7% of control (n = 7), respectively (Fig.2C). The effect of 4C3HPG began within one respiratory cycle (<10 sec) after drug application and reached peak within 1 min. After washout, the inspiratory drive current returned to the control level within 5–8 min (Fig. 2D). Concurrent with the reduction of inspiratory drive current, a decrease in inspiratory discharges in C4 ventral roots occurred (Fig. 2A). The effect of 4C3HPG on C4 roots had a time course similar to that of the effect on inspiratory current of PMNs (Fig.2A).

Fig. 2.
Fig. 2.

Activation of group-II mGluRs depresses synaptic transmission to and output from PMNs. A,B, Local application of the agonist 4C3HPG (500 μm) simultaneously decreased the activity of C4 ventral roots (A) and the inspiratory drive current of a PMN that was voltage-clamped at the end-expiratory potential of −60 mV (B). Inset, The superimposed traces are averages of six consecutive inspiratory drive currents of a PMN (Im ) and integrated inspiratory discharges of C4 roots (∫C4) in control conditions and during the period of peak effect after drug application.C, Summary of effects of 4C3HPG (500 μm, local) on peak amplitude (Amp) and charge transfer of inspiratory drive currents is shown. Vertical bars are averages of six successive inspiratory drive currents during peak effect of the drug pooled from seven preparations. Error bars indicate SEM. An asterisk indicates a significant difference (p < 0.05; t test) from control values. D, Time course of peak inspiratory drive currents in response to 4C3HPG (500 μm, local) is shown. Each data point is the average of three consecutive peak inspiratory drive currents expressed as the percentage of the control value.

The role of group-III mGluRs was also examined.l-AP4, an agonist for group-III mGluRs (Bushell et al., 1995; Tones et al., 1995), inhibits synaptic transmission to PMNs (Liu et al., 1990). l-AP4 potently reduced the inspiratory current of PMNs (Fig. 3) without any effect on the baseline current. The peak inspiratory current was reduced to 51 ± 6% (n = 6) of control by 50 μml-AP4. Concurrent with the reduction of inspiratory current of PMNs, a decrease in inspiratory discharges in C4 ventral roots occurred in response to l-AP4 (data not shown). In the presence of MSOP (1 mm, local), an antagonist for group-III mGluRs (Thomas et al., 1996), the effect ofl-AP4 was diminished; 50 μml-AP4 reduced inspiratory current only to 88 ± 7% (n = 6; Fig. 3).

Fig. 3.
Fig. 3.

Activation of group-III mGluRs reduces PMN inspiratory drive currents. A, Locally appliedl-AP4 (50 μm) potently reduced inspiratory drive currents. This effect was effectively blocked by the antagonist MSOP. Local application of MSOP (1 mm) began 5 min beforel-AP4 (50 μm, local) application and continued during the course of the l-AP4 test.Traces are the averages of six consecutive inspiratory drive currents in each condition. B, Summary of thel-AP4 (50 μm, local) effect on peak inspiratory drive currents with and without concurrent application of MSOP (1 mm, local) is shown. Error bars indicate SEM. Anasterisk indicates a significant difference (p < 0.05; t test) from control values. A pound symbol indicates a significant difference (p < 0.05; ttest) from values obtained from the l-AP4 condition.

There were no changes in respiratory frequency with either 4C3HPG (Fig.2) or AP-4 (data not shown) applied locally to the spinal cord.

Effects of elevation of intracellular cAMP on mGluR-mediated actions

The various mGluRs are coupled to different second messenger cascades (Masu et al., 1991; Abe et al., 1992; Aramori and Nakanishi, 1992). To confirm further the distinction of the effects on PMN excitability of group-I and group-II/-III receptor subtypes, we examined the involvement of specific second messenger pathways. The membrane-permeable cAMP analog 8-Br-cAMP was used to elevate intracellular cAMP concentration so that any effects mediated via the cAMP cascade would be masked or occluded.

In the presence of 8-Br-cAMP (0.8–1.2 mm) in the spinal bath of a partitioned chamber, the ability of both 4C3HPG andl-AP4 to reduce inspiratory-modulated activity in the C4 roots was greatly attenuated (Fig. 4). Thus, 4C3HPG (500 μm) could only reduce C4 root discharges to 87 ± 6% (n = 6) of control, compared with 40 ± 7% before 8-Br-cAMP treatment (Fig.4A,B), and l-AP4 (50 μm) could only reduce C4 root discharges to 77 ± 7% (n = 6) of control, compared with 42 ± 9% before 8-Br-cAMP treatment (Fig. 4C,D). In contrast, the effect of DHPG was unaffected by 8-Br-cAMP (n = 4), i.e., it continued to elicit tonic discharges in C4 ventral roots (Fig. 5).

Fig. 4.
Fig. 4.

Elevation of intracellular cAMP attenuates the effects mediated by group-II and group-III mGluRs. A,C, Time courses of changes of C4 root inspiratory discharges in response to local application of 4C3HPG (500 μm; A) and l-AP4 (50 μm; C) with and without 8-Br-cAMP (1 mm, bath) treatment. Effects of both 4C3HPG andl-AP4 on inspiratory discharges were significantly attenuated by 8-Br-cAMP. Bath application of 8-Br-cAMP began 8 min before 4C3HPG or l-AP4 application and continued during the course of each agonist’s application. Each data point is the average of three consecutive integrated inspiratory discharges expressed as the percentage of the control value. B, D, Pooled data from six preparations showing attenuated effects of 4C3HPG (B) and l-AP4 (D) on C4 root inspiratory activity by 8-Br-cAMP. Error bars indicate SEM. An asterisk indicates a significant difference (p < 0.05;t test) from control values. A pound symbol indicates a significant difference (p < 0.05; t test) from values obtained from the 4C3HPG or l-AP4 condition.CTRL, Control.

Fig. 5.
Fig. 5.

Lack of effect of intracellular cAMP elevation on the effect of group-I mGluR activation. A, Local application of DHPG (200 μm) caused tonic discharges in C4 ventral roots. B, This effect was unaltered by treatment with 8-Br-cAMP. C4, Raw trace of C4 root activity is shown. ∫C4, Integrated trace of C4 root activity is shown. Protocols described in Figure 4 were used for the 8-Br-cAMP treatment. The horizontal dashed line inB indicates the period of 8-Br-cAMP treatment.

Differential effects of distinct mGluR subtypes on postsynaptic membrane properties

To elucidate the ionic mechanisms underlying the effects on baseline membrane current and inspiratory drive current mediated by the various mGluR subtypes, we examined the PMN current–voltage (I–V) relationship before and after drug treatment after synaptic isolation by TTX (1 μm, bath; Fig.6).

Fig. 6.
Fig. 6.

Differential effects of distinct mGluR subtypes on postsynaptic membrane properties. A, MembraneI–V relationship before and after application of DHPG (30 μm, bath). The I–V curve was obtained by plotting current changes (averaged steady-state current values at 5–10 msec before offset of voltage step) against membrane potentials. Currents were generated by a series of command voltage pulses. Pulse step size was 5 mV; pulse width was 100 msec; and pulse frequency was 2 Hz. Note that the membrane input resistance increased in the DHPG condition as indicated by the reduced slope of the I–Vplot. B, I–V relationship, obtained by subtracting the I–V relationship during DHPG treatment from that in the control condition, for the DHPG-induced inward current (IDHPG). These experiments were performed in the presence of TTX (1 μm, bath).C, D, Membrane I–Vrelationships before and after applications of 4C3HPG (50 μm, bath; C) and l-AP4 (5 μm, bath; D).

DHPG increased input resistance, as indicated by the reduced slope of the I–V curve (Fig. 6A). The membrane input resistance at the resting potential (−60 to −75 mV) increased to 159 ± 8% of control (n = 6) after DHPG treatment (30 μm, bath). The I–V relationship for IDHPG (Fig. 6B) was obtained by subtracting the I–V relationship during DHPG treatment from that obtained under control conditions (Fig.6A). IDHPG decreased linearly with hyperpolarizing potentials (Fig. 6B). A reversal potential of −102 ± 6 mV for IDHPG was seen in four of six PMNs within the testing voltage range (−50 to −120 mV).

To examine the possible postsynaptic actions of group-II and group-III mGluRs on PMNs, we also examined the effects of 4C3HPG (n = 5) and l-AP4 (n = 4). In contrast to the group-I agonist DHPG, neither 4C3HPG norl-AP4 had a significant effect on the I–Vrelationship over the test voltage range (−50 to −120 mV) (Fig.6C,D). There was no detectable change in membrane input resistance after 4C3HPG or l-AP4 (Fig.6C,D).

Site of mGluR actions affecting inspiratory drive currents

The reduction of the inspiratory drive current of PMNs caused by group-II and group-III mGluR agonists could result from actions either at presynaptic sites to decrease glutamate release or at postsynaptic sites to affect the responsiveness of ionotropic glutamate receptors to released glutamate. To investigate the underlying mechanism(s), we examined the effects of these agonists on the amplitude and frequency of mEPSCs. After treatment with TTX (1 μm, bath), PMNs exhibit spontaneous mEPSCs (Fig.7A) (Liu and Feldman, 1992;Dong and Feldman, 1995a). These events were collected from a 20–25 min control period (Fig. 7B, top) and subsequently 25–30 min during drug application (Fig. 7B,bottom). The time interval between successive mEPSCs and their peak amplitude were used to construct cumulative interval and amplitude histograms (see Fig. 7C,D).

Fig. 7.
Fig. 7.

Effect of group-II and group-III agonists on mEPSCs in PMNs. A, Raw trace with higher temporal resolution showing typical mEPSCs after bath application of TTX (1 μm). B, Top, Rawtrace showing mEPSCs before drug treatment.Bottom, Decrease of mEPSC frequency after 4C3HPG (30 μm, bath) treatment. C, Cumulative (Cum) interval (Intvl) histograms of mEPSCs from the cell represented in B before (1012 events; gray curve) and after (810 events; black curve) bath application of 4C3HPG, which induced a significant (p < 0.01) rightward shift in the cumulative distribution of mEPSC intervals (i.e., a decrease in mean EPSC frequency). D, Cumulative amplitude (Amp) histograms of mEPSCs from the same data sets shown in C. Note that there was no significant (p > 0.05) difference in the amplitude distributions between control and 4C3HPG conditions. Statistical significance for the difference between distributions was assessed by the Kolmogorov–Smirnov test. E, F, Summary of 4C3HPG (E) and l-AP4 (F) effects on the amplitude (Amp) and frequency (Freq) of mEPSCs. Each value (mean ± SEM) was obtained by averaging the percentage changes of mean amplitude or interval (as the reciprocal of frequency) from cells tested with 4C3HPG (30 μm, bath; n = 5) orl-AP4 (5 μm, bath; n = 4). An asterisk indicates a significant difference (p < 0.05; t test) from control values.

The group-II agonist 4C3HPG caused a significant decrease in the frequency of mEPSCs (Fig. 7C). The decrease is indicated by the shift toward longer values of the interval histogram for 4C3HPG compared with the control histogram. In contrast, the amplitude of mEPSCs was not significantly altered by 4C3HPG, as indicated by overlapping cumulative amplitude histograms (Fig. 7D). The mean frequency of mEPSCs was 74 ± 11% of control (n = 5) after 4C3HPG (30 μm, bath) treatment (Fig. 7E), whereas the mean amplitude of mEPSCs was not significantly altered (97 ± 9%; n = 5) by 4C3HPG (Fig. 7E).

Similarly, the group-III agonist l-AP4 significantly decreased the frequency of mEPSCs while not affecting their amplitude. The mean frequency of mEPSCs after l-AP4 (5 μm, bath) was reduced to 69 ± 10% (n = 4), whereas the mean amplitude was not significantly altered (96 ± 11%; n = 4; Fig.7F).

Endogenous activation of mGluRs shapes the inspiratory drive to PMNs

To determine the endogenous activation of mGluRs and their physiological roles in synaptic transmission of inspiratory drive to PMNs, we examined the effects of their antagonists. The group-I mGluR antagonist AIDCA, applied locally over the PMN pool (2 mm), significantly (p < 0.01) reduced the peak inspiratory drive current (Fig.8A,D) to 84 ± 6% (n = 5) of control. Concurrent with the decrease of PMN inspiratory drive currents, a reduction of C4 root activity by AIDCA occurred (data not shown). The effect of AIDCA began 25–30 sec after the onset of drug application and took 4–5 min to peak (Fig. 8D). After washout, inspiratory activity returned to the control level within 10–15 min.

Fig. 8.
Fig. 8.

Endogenous activation of mGluRs during the inspiratory phase revealed by antagonists for different subgroups of mGluRs. A, Attenuation of inspiratory drive current of a PMN by the group-I mGluR antagonist AIDCA (2 mm, local).B, Enhancement of inspiratory drive current of a PMN by the group-II mGluR antagonist EGLU (2 mm, local).C, Increase of inspiratory activity in C4 ventral roots by the group-III antagonist MSOP (2 mm, local).Traces are the averages of six consecutive inspiratory drive currents (Im ; A,B) or six integrated inspiratory discharges in C4 roots (∫C4; C) before and after drug application.D, E, Time courses of changes of inspiratory currents in response to locally applied AIDCA (D) and EGLU (E). Each data point is the average of three consecutive peak inspiratory currents expressed as the percentage of the control value.

In contrast, antagonists for group-II and group-III mGluRs enhanced the inspiratory activity of PMNs. EGLU, an antagonist for group-II mGluRs, increased inspiratory current in PMNs (Fig.8B,E) and in C4 root activity (data not shown). Locally applied EGLU (2 mm) increased inspiratory current by 31 ± 7% (n = 5) above control. The time course of the effect was similar to that of AIDCA (Fig. 8E). An antagonist for group-III, MSOP, also increased inspiratory drive current of PMNs (data not shown) and their output as C4 root activity (Fig. 8C).

DISCUSSION

This study demonstrates that inspiratory-modulated release of glutamate can activate various subtypes of mGluRs to affect differentially the excitability of PMNs. Using specific agonists, we identified mGluR subtypes mediating different effects. We propose that group-I mGluRs mediate the increase of excitability and that group-II and group-III mGluRs are responsible for the decrease of synaptic transmission.

Postsynaptic group-I mGluRs mediate an increase in PMN excitability

Activation of group-I mGluRs results in an increase in PMN excitability characterized by enhanced firing in response to inspiratory drive input. We found that the associated cellular responses, such as the production of an inward current and the increase in input resistance, persisted when synaptic transmission was blocked; these responses were not associated with any change in synaptic current. In addition, these effects were induced only by the agonist for group-I mGluRs and not by the agonists for the other groups. Taken together, our data suggest that postsynaptic group-I mGluRs mediate the increase of PMN excitability.

High levels of mGluR1 and mGluR5 mRNA expression are present in rat spinal cord (Valerio et al., 1997). Although there is a lack of information regarding the cellular localization of mGluRs in the phrenic nucleus, in many other brain areas group-I mGluRs are mainly localized postsynaptically (Martin et al., 1992; Baude et al., 1993;Lujan et al., 1996; Shigemoto et al., 1997), where they increase neuronal excitability (Davies et al., 1995; Batchelor et al., 1997;Schoppa and Westbrook, 1997; Schrader and Tasker, 1997) consistent with our conclusion that postsynaptic group-I mGluRs increase PMN excitability. Our finding is in agreement with studies in other brain regions. Activation of postsynaptic group-I mGluRs increases firing of hypothalamic neurons (Schrader and Tasker, 1997) and induces a depolarization or an inward current and an associated increase in input resistance in hippocampal CA1 pyramidal neurons (Davies et al., 1995) and olfactory bulb mitral cells (Schoppa and Westbrook, 1997).

The effect of DHPG on PMNs resembles that elicited by 1S,3R-ACPD (Dong et al., 1996), including the production of an inward current that reverses at a potential close to the estimated EK+ (−95 mV) and an associated decrease in membrane conductance. Elevation of extracellular [K+] shifts the reversal potential of the 1S,3R-ACPD–induced inward current (IACPD) in the same direction as theEK+ change. In addition, the K+ channel blocker Ba2+ occludes the effects of 1S,3R-ACPD. We concluded thatIACPD results principally from the blockade of a Ba2+-sensitive K+ conductance (Dong et al., 1996). This mechanism may also underlie DHPG effects because the action of 1S,3R-ACPD and DHPG on the postsynaptic membrane of PMNs is very likely mediated by the same mGluR group, i.e., group-I, according to the following evidence. (1) The effects produced by 1S,3R-ACPD and DHPG on the postsynaptic membrane of PMNs are quite similar, suggesting that the same signal transduction mechanisms are involved. (2) DHPG is highly selective for group-I over group-II and group-III mGluRs. (3) Although 1S,3R-ACPD can interact with group-II and/or group-III mGluRs, their agonists did not affect postsynaptic membrane properties of PMNs. We conclude that the postsynaptic component of 1S,3R-ACPD actions described previously was mediated via group-I mGluRs. Therefore, we suggest that blockage of a Ba+-sensitive K+conductance mediates the increase in PMN excitability by group-I mGluRs. In addition, changes in some other conductance(s) may be also involved in group-I mGluR-mediated action [see Dong et al. (1996), their Discussion].

Presynaptic group-II and group-III mGluRs mediate a decrease of synaptic current

Activation of group-II or group-III mGluRs decreased inspiratory drive current in PMNs. This effect was not observed when the agonist for group-I mGluRs was applied. To confirm further the involvement of group-II or group-III mGluRs, their second messenger pathways were examined. Group-II and group-III mGluRs are linked to cAMP (Tanabe et al., 1992, 1993; Nakajima et al., 1993; Okamoto et al., 1994; Saugstad et al., 1994; Duvoisin et al., 1995), whereas group-I mGluRs are coupled to phospholipase C (Masu et al., 1991; Abe et al., 1992;Aramori and Nakanishi, 1992). Elevation of intracellular cAMP concentration would mask or occlude an effect mediated via cAMP cascades. Pretreatment with the membrane-permeable cAMP analog 8-Br-cAMP occluded the reduction of inspiratory drive by agonists for group-II and group-III, confirming that group-II and group-III mGluRs mediate the decrease of synaptic transmission of inspiratory drive.

The reduction of inspiratory drive current appears to result from a decrease of transmitter release because of activation of mGluR autoreceptors located at presynaptic terminals of bulbospinal inspiratory neurons onto PMNs. First, our mEPSC analysis showed that the frequency of mEPSCs was significantly reduced by both group-II and group-III agonists, whereas the mEPSC amplitude was unaffected. Because mEPSC frequency is dependent on transmitter release probability (Fatt and Katz, 1952; Redman, 1990), we assume that its reduction is a presynaptic action of a group-II or group-III agonist to decrease transmitter release from bulbospinal terminals onto PMNs. On the other hand, changes in mEPSC amplitude could result from a postsynaptic action of test drugs to affect the postsynaptic sensitivity to the endogenously released transmitter (Fatt and Katz, 1952; Redman, 1990;Kullmann and Siegelbaum, 1995). The fact that mEPSC amplitude was unaffected by either group-II or group-III agonists suggests a lack of their postsynaptic action. Although the origin of these mEPSCs was not identified, it is likely that the presynaptic terminals producing the mEPSCs include those of bulbospinal inspiratory neurons. Therefore, we extend our conclusion drawn from the mEPSCs to unitary EPSCs comprising the endogenous excitatory inspiratory drive current. However, caution must be taken when extrapolating the conclusions from mEPSC analysis of PMNs to inspiratory drive current. One important difference between spontaneous mEPSCs and evoked synaptic currents is that mEPSCs do not require Ca2+ influx (Scanziani et al., 1992; Scholz and Miller, 1992), which must be considered because activation of presynaptic mGluRs has been postulated to reduce Ca2+ influx (Stefani et al., 1994; Glaum and Miller, 1995; Yoshino and Kamiya, 1995). The reduction in mEPSC frequency we observed indicates that a Ca2+-independent mechanism, such as interference with the secretion cascade (Hayashi et al., 1993; Gereau and Conn, 1995; Scanziani et al., 1995; Tyler and Lovinger, 1995; Schoppa and Westbrook, 1997), is involved. Such a mechanism could also attribute, if not exclusively, to the inhibition of evoked transmitter release. Regardless of the precise mechanism, the decrease in transmitter release from bulbospinal presynaptic terminals by presynaptic group-II and group-III mGluRs leads to the reduction of inspiratory drive current.

Second, no alterations in steady-state membrane current or the input resistance of PMNs were produced by the agonist for group-II or group-III mGluRs, indicating that the decrease of inspiratory drive current by activation of these receptors is not caused by the shunting of postsynaptic currents.

Third, the decrease in synaptic current is most likely caused by direct action of drugs on the synapses of bulbospinal inspiratory terminals to PMNs rather than by an action on putative spinal interneurons relaying the descending inspiratory drive to PMNs. Bulbospinal transmission of inspiratory drive to PMNs seems to be mediated primarily by a monosynaptic pathway (Ellenberger and Feldman, 1988; Berger et al., 1989; Ellenberger et al., 1990; Lipski et al., 1994) and not by spinal interneurons (Davies et al., 1985; Lipski and Duffin, 1986; Palisses et al., 1989; Bellingham and Lipski, 1990; Grelot et al., 1993) (X.-W. Dong and J. L. Feldman, unpublished observations). In addition, when PMNs were isolated by TTX, group-II or group-III mGluR agonist continued to affect the frequency of mEPSCs. Therefore, drug effects seem to be attributable to direct action on impinging presynaptic terminals.

In many brain regions, group-II and group-III mGluRs appear predominantly localized in presynaptic terminals (Shigemoto et al., 1995, 1996, 1997). The presynaptic distribution is consistent with their physiological roles in modulating synaptic transmission. These mGluRs can inhibit transmitter release in areas such as the hippocampus (Forsythe and Clements, 1990; Baskys and Malenka, 1991; Gereau and Conn, 1995; Schrader and Tasker, 1997), thalamus (Salt and Eaton, 1995), hypothalamus (Schrader and Tasker, 1997), olfactory bulb (Trombley and Westbrook, 1992; Schoppa and Westbrook, 1997), and trigeminal motor nucleus (Del Negro and Chandler, 1998). We conclude that this is also the case for bulbospinal transmission of inspiratory drive to PMNs.

Endogenous activity and functional significance of mGluRs

We observed significant changes in the inspiratory-modulated activity of PMNs by antagonists for each of three groups of mGluRs, suggesting endogenous activation of all groups. The reduction of inspiratory drive current by the mGluR1 antagonist AIDCA suggests that mGluR1s, in addition to various ionotropic receptors (Liu et al., 1990;Greer et al., 1991), are activated by endogenously released glutamate during the inspiratory phase and the resultant current contributes to the total inspiratory drive current. The mGluR1-mediated inward current will produce an incremental increase in the inspiratory-modulated depolarization. The concurrent increase in membrane resistance should also increase this depolarization. Our finding that the EPSCs of PMNs are mediated by glutamate acting at both ionotropic and group-I mGluRs is consistent with observations in other brain areas. In hippocampal CA3 pyramidal cells, when the fast ionotropic response is blocked pharmacologically, stimulation of mossy fibers produces a depolarizing postsynaptic potential associated with a decrease in membrane conductance (Charpak and Gähwiler, 1991; Gerber et al., 1993). This EPSP is greatly reduced by a mGluR antagonist methyl-4-carboxyphenylglycine (Gerber et al., 1993). mGluR1s also mediate responses of thalamic neurons to noxious thermal somatosensory stimuli (Salt and Turner, 1998) and EPSPs at parallel fiber–Purkinje cell synapses in the cerebellum (Batchelor et al., 1997).

The enhancement of inspiratory drive current or discharges of PMNs by antagonists for group-II and group-III mGluRs is presumably caused by the blockade of presynaptic receptors. This finding suggests that, at least in this in vitro preparation, bulbospinal transmission is attenuated by endogenous activation of presynaptic group-II and group-III mGluRs. Such a presynaptic action may provide a rapid negative (autoregulatory) feedback to reduce further glutamate release under physiological conditions.

In summary, three groups of mGluRs are all functionally expressed in the synapses of bulbospinal inspiratory neuron terminals to PMNs. These receptors are activated during endogenous inspiratory drive transmission to modulate this process. Along with other modulatory systems, such as 5-HT (Lindsay and Feldman, 1993) and adenosine (Dong and Feldman, 1995a), different groups of mGluRs function to ensure that the synaptic transmission of inspiratory drive to spinal respiratory motoneurons is well adjusted to produce the appropriate respiratory motor output under widely varying physiological conditions with different ventilatory demands.

Footnotes

  • This work was supported by the National Institutes of Health Grant NS24742. We thank Dr. Didier Morin for participating in the early experimental studies.

    Correspondence should be addressed to Dr. Jack L. Feldman, Department of Neurobiology, University of California, Los Angeles, Box 951763, Los Angeles, CA 90095-1763.

    Dr. Dong’s present address: Schering-Plough Research Institute, 2015 Galloping Hill Road, Kenilworth, NJ 07033.

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Distinct Subtypes of Metabotropic Glutamate Receptors Mediate Differential Actions on Excitability of Spinal Respiratory Motoneurons
Xiao-Wei Dong, Jack L. Feldman
Journal of Neuroscience 1 July 1999, 19 (13) 5173-5184; DOI: 10.1523/JNEUROSCI.19-13-05173.1999
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