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Leak channels regulate neuronal activity and excitability. Determining which leak channels exist in neurons and how they control electrophysiological behavior is fundamental. Here we investigated TASK channels, members of the two-pore domain K+ channel family, as a component of the K+-dominated leak conductance that controls and modulates rhythm generation at cellular and network levels in the mammalian pre-Bötzinger complex (pre-BötC), an excitatory network of neurons in the medulla critically involved in respiratory rhythmogenesis. By voltage-clamp analyses of pre-BötC neuronal current-voltage (I-V) relations in neonatal rat medullary slices in vitro, we demonstrated that pre-BötC inspiratory neurons have a weakly outward-rectifying total leak conductance with reversal potential that was depolarized by ~4 mV from the K+ equilibrium potential, indicating that background K+ channels are dominant contributors to leak. This K+ channel component had I-V relations described by constant field theory, the conductance was reduced by acid and was augmented by the volatile anesthetic halothane, which are all hallmarks of TASK. We established by single-cell RT-PCR that pre-BotC inspiratory neurons express TASK-1 and in some cases also TASK-3 mRNA. Furthermore, acid depolarized and augmented bursting frequency of pre-BötC inspiratory neurons with intrinsic bursting properties. Microinfusion of acidified solutions into the rhythmically active pre-BötC network increased network bursting frequency, halothane decreased bursting frequency, and acid reversed the depressant effects of halothane, consistent with modulation of network activity by TASK channels. We conclude that TASK-like channels play a major functional role in chemosensory modulation of respiratory rhythm generation in the pre-Bötzinger complex in vitro.
Leak or background channels determine neuronal resting membrane potentials, regulate excitability, and control electrophysiological behavior. Multiple channels mediate leak currents, including channels with mixed cationic permeabilities (Liu et al., 2007) and specific types of K+ channels such as TASK channels, members of the family of two-pore domain K+ (K2P) channels (Lesage and Lazdunski, 2000). TASK-1 and TASK-3, two forms of TASK present in mammalian brain (Medhurst et al., 2001; Mulkey et al., 2007), like other background channels, are targets for neuromodulation (Tally et al., 2000; Mathie, 2007). Identifying which leak channels exist in different neurons and how they regulate electrophysiological behavior including via neuromodulation is fundamental.
Here we identified TASK-like channels and examined their role in regulation of rhythm generation within the brainstem respiratory pre-Bötzinger complex (Smith et al., 1991; Gray et al., 2001), a region of the mammalian medulla containing a heterogeneous excitatory network that is the substrate for inspiratory rhythm generation (Smith et al., 2000; Feldman and Del Negro, 2007). This network has autorhythmic properties (Johnson et al., 2001) and remains active in neonatal rodent medullary slice preparations, allowing analyses of cellular and network mechanisms of rhythmogenesis in vitro (Smith et al., 1991; Koshiya and Smith, 1999; Del Negro et al., 2001). We have proposed (Butera et al., 1999a,b) and found experimentally (Koizumi and Smith, 2008) that a K+-dominated leak conductance plays a fundamental role in generation and control of pre-BötC rhythmic activity in vitro.
Channels mediating this conductance, however, have not been identified. We hypothesized that TASK channels contribute based on known biophysical and chemosensitive properties. TASK channels have I-V relations that fit constant field theory for simple electro-diffusion through an open K+-selective pore (Leonoudakis et al., 1998), consistent with our observations of pre-BötC neuronal leak I-V properties (Koizumi and Smith, 2008). Furthermore, the pre-BötC network is hypothesized to have chemosensitive properties (Solomon et al., 2000; Nattie, 2001). TASK channels close in response to extracellular acidification (Duprat et al., 1997; Rajan et al., 2000). A further chemosensitivity is that TASK channels open in response to halothane (Talley and Bayliss, 2002) and other volatile anesthetics (Bayliss et al., 2003). Thus TASK may contribute to pre-BötC neuronal pH-related chemosensory properties and suppression of rhythmic breathing by volatile anesthetics. Modulation of pre-BötC leak currents by serotonin and substance P, two important neuromodulators of rhythmogenesis, is mediated in part by TASK-like and by non-selective cationic NALCN-like conductance components (Lu et al., 2007, 2009; Hayes and Del Negro, 2007; Ptak et al., 2009), suggesting a critical neuromodulatory role of TASK.
The four properties of TASK channels, selectivity for K+, I-V relations described by constant field theory, closure to extracellular acid, and opening to halothane, differentiate TASK from all other known channels. We used these properties to probe for TASK channels in pre-BötC inspiratory neurons in rhythmically active neonatal rat brainstem slices in vitro. Augmentation of TASK-like conductance by halothane down-regulated, and reductions in conductance by extracellular acid augmented, rhythm generation at cellular and network levels, implying a functional role of TASK channels in pre-BötC chemoreception and respiratory rhythm generation in vitro.
Transverse slices (250 – 350 μm thick) of medulla oblongata were cut from Sprague-Dawley neonatal (P0 – P4) rats to contain the pre-BötC and rostral end of the hypoglossal (XII) motor nucleus including XII nerve rootlets as previously described (Koshiya and Smith, 1999; Koizumi and Smith, 2008). All animal use procedures were approved by the institutional Animal Care and Use Committee of NINDS, NIH (approved ASP #1154-06). The caudal surface of the slice was cut through the caudal pre-BötC for imaging and recording neuronal activity. The slice was oriented caudal end up in a recording chamber (0.2 ml) mounted on the stage of an upright microscope, anchored in the chamber by nylon fibers attached to an overlying platinum ring, and superfused (4 ml/min) with artificial cerebrospinal fluid (aCSF) containing (in mM) 124 NaCl, 25 NaHCO3, 3 KCl, 1.5 CaCl2, 1.0 MgSO4, 0.5 NaH2PO4, 30 D-glucose and antibiotics (500 units/l penicillin, 0.5 mg/l streptomycin and 1 mg/l neomycin), equilibrated with 95% O2 and 5% CO2 (pH = 7.35 – 7.40 at 27 °C). Rhythmic respiratory network activity recorded from XII nerves was maintained by elevating the superfusate K+ concentration (8 mM).
Pharmacological agents [tetrodotoxin (TTX, Sigma-RBI, St. Louis, MO), ZD7288 (Tocris Bioscience, Bristol, UK), 6-cyano-7-nitroquinoxaline-2,3-dione disodium (CNQX, Sigma), barium chloride (Ba2+, Sigma), tetraethyl ammonium chloride (TEA, Sigma), and/or cadmium chloride (Cd2+, Sigma)], were dissolved in the standard perfusion solution with elevated K+ concentration. Acidified aCSF (pH 7.2, 7.0, 6.8, 6.5, 6.0) was prepared by decreasing the concentration of NaHCO3 in the aCSF; osmolarity was maintained by increasing the concentration of NaCl. The aCSF was equilibrated by continuous bubbling with halothane delivered by a calibrated vaporizer (Fluotec, Surgivet, Waukesha, WI), with vaporizer settings of 0.25% – 2.0%. From our functional assays this produced effective concentrations in the slice bathing solution that progressively and reversibly depressed pre-BötC neuronal or network rhythmic activity in a concentration-dependent manner, and also reversibly augmented leak conductance as found for other CNS neurons where the same percentage gas compositions were employed and gas chromatographic analysis demonstrated aqueous anesthetic concentrations within expected ranges for anesthetic efficacy (e.g. Siros et al., 2000). In some experiments the aCSF was equilibrated with isoflurane delivered by a separate calibrated vaporizer (Isotec, Surgivet) with vaporizer settings of 0.5% – 2.0%. In all cases the perfusion solutions were delivered to the bath (4 ml/min) through a short segment of gas-impermeable tubing to minimize loss of the anesthetic. We therefore denote the anesthetic compositions of our slice bathing solution by the percentage of vaporized anesthetic equilibrated with the perfusate.
Acidified aCSF or halothane equilibrated aCSF, prepared as above, was loaded into a polished glass pipette (~10 μm tip diameter), positioned 100 – 200 μm deep into the core of the pre-BötC (depending on slice thickness) (Fig. 1 below), and continuously infused convectively, to minimize local concentration gradients, by applying low pressure (~10 – 20 mmHg) to the pipette with a precision pressure control and valve system (Picospritzer-IID, General Valve Corp, Fairfield, NJ, and 2PK+ Pressure Controller, ALA Scientific Instruments, Inc. Westbury, NY). This system allowed us to precisely control convective microdelivery of anesthetic-containing or acidic aCSF locally within the imaged locus of pre-BötC network activity (below, Koizumi and Smith, 2008). For the typical microinfusion rate (10 nl-min-1) employed, we estimate that the infusate would spread by convection and have effective concentrations over a region of ~200 – 300 μm in diameter, which would encompass the pre-BötC region on each side (Fig. 1). This was tested in some experiments by microinfusing the halothane-or acid-containing solution at the same rate adjacent to the pre-BötC by positioning the infusion pipette tip at the same depth in the tissue but 200 μm from the boundary of the imaged pre-BötC region. These infusions did not cause any perturbations of network activity, indicating that we could achieve site-specificity with our microinfusion procedures when applied to the pre-BötC.
We imaged rhythmic Ca2+ fluorescence transients of inspiratory neurons to map the location of the pre-BötC at the level of population activity for microinfusion experiments (Koizumi and Smith, 2008) and individual neurons for whole-cell patch-clamp recording. Methods for retrograde labeling of pre-BötC neurons with Ca2+-sensitive dye and imaging were as previously described (Koshiya and Smith, 1999; Koizumi et al., 2008). Briefly, membrane-permeant Ca2+-sensitive dye, Calcium Green-1 AM (CaG; Molecular Probes, Eugene, OR, 50 μg), dissolved in 5 μl of DMSO containing 25 μg of pluronic F-127 (BASF) and dispersed in 10 μl of ACSF, was microinjected with a glass pipette (~10 μm tip diameter) into the slice near the midline to retrogradely label bilaterally pre-BötC neurons overnight (8 – 12h). CaG-labeled inspiratory neurons were visualized with a fixed-stage upright microscope (Axioskop-FS1or FS2, Zeiss, Thornwood, NY) with a 75 W xenon epi-illuminator, optical filters (excitation 485 nm, emission 530 nm, and beam splitter 505 nm, Omega Optical) and a 63X water-immersion objective (Zeiss Achroplan, N.A. 0.95). Fluorescence images were captured with a CCD camera fiber-optically coupled to a fluorescence image-intensifying camera (ICCD-1000F, VideoScope International, Dulles, VA) and recorded on videotape and digitized together with electrophysiological signals. Changes in fluorescence intensity (ΔF/F) were detected in real time with an image processor (ARGUS 20, Hamamatsu Photonics, Bridgewater, NJ) and quantified off-line after digitizing images using an audio-video board (SONY Media Converter). Inspiratory population and single neuron “flash” images were obtained by subtracting base-line CaG fluorescent images from images acquired during peak inspiratory activity with an image processor in real time and displayed in pseudocolor. Simultaneous videomicroscopic infrared differential interference contrast (IR-DIC) imaging was done using 900 nm infrared illumination, a wide spectrum polarizer (Melles Griot, Rochester, NY), and an 850 – 950 nm analyzer (Polarcor, Corning, NY). The IR-DIC image was captured with an extended IR Newvicon camera (Hamamatsu Photonics), and enhanced with the ARGUS 20 in real time. For dual imaging, the Newvicon and ICCD cameras were mounted on a dual-port imaging head incorporating a dichroic beam splitter (700 nm, Zeiss), and images were aligned by reverse scanning and scan range shifting of the Newvicon camera.
XII motoneuron population activity, used to monitor inspiratory network activity in the slices (Fig. 1 below), was recorded with fire-polished glass suction electrodes (60 – 90 μm inner diameter), amplified (5,000 – 10,000X, CyberAmp 380, Axon Instruments), band-pass filtered (0.3 – 2 kHz), digitized (10 kHz) with an AD converter (Power Lab, AD Instruments, Inc., Colorado Springs, CO), and then rectified and integrated (∫XII) by either an analog integrator or digitally via software (Chart software, ADInstruments). Measurements of parameters of network population activity (inspiratory population burst frequency) were made offline with custom automated algorithms in Chart software (AD Instruments) and Igor Pro (Wavemetrics, Portland, OR) for XII inspiratory burst detection and hand-checked for accuracy. All data presented as burst frequency were first analyzed by computing burst period, defined as the interval from onset to onset of consecutive inspiratory bursts.
Voltage- and current-clamp data obtained from whole-cell patch-clamp pipette electrodes was recorded with a HEKA (HEKA Electronics Inc., Mahone Bay, Nova Scotia, Canada) EPC-9 amplifier controlled by Pulse or PatchMaster software (HEKA; 2.8 kHz low-pass filter). Borosilicate recording electrodes (4 – 6 MΩ), positioned with microdrives (Sutter Instrument, Novato, CA, or SD Instruments, Grants Pass, OR), contained (in mM): 130.0 K-gluconate, 10.0 Na-gluconate, 4.0 NaCl, 10.0 HEPES, 4.0 Mg-ATP, 0.3 Na-GTP, and 4.0 sodium phosphocreatine, adjusted with NaOH to match the intracellular pH (7.3, Filosa et al., 2002; Putnam et al., 2004). Rhythmically active neurons were identified by CaG fluorescence transients as described above. In some experiments were indicated, we alternatively employed blind whole-cell patch-clamp recording to include in the sample neurons deeper in the slice (>90 μm below the slice surface) beyond the limits of optical resolution. In all cases measured potentials were corrected for the liquid junction potential (−10 mV). To identify intrinsic oscillatory bursting neurons, excitatory synaptic transmission was blocked with 20 μM CNQX or in by the calcium channel blocker Cd2+ (200 μM). To control for non-K2P currents during measurement of cellular leak conductance, in some experiments sodium channels as well as synaptic currents were blocked with TTX (1 μM), inwardly rectifying K+ conductance (Kir) was blocked with barium (200 μM), Kv + channels with TEA (10 mM), voltage-gated Ca2+ channels with cadmium (200 μM), and h-current (Ih) with ZD7288 (100 μM) (Shin et al., 2001), all dissolved in the slice perfusate solution.
Measurements of neuronal burst frequency in current clamp were made off line with Chart software and Igor Pro. All data presented as neuronal burst frequency were analyzed by computing burst period with spike detection algorithms and subsequent computation of burst frequency was done similar to that for population activity as described above.
Voltage-dependence of whole-cell currents was analyzed from voltage-clamp data using Pulsefit, Chart, and Igor Pro software. Neuronal membrane leak conductance (gLeak) was determined from measurements of leak currents using slow voltage ramps (30 mV/s, −110 mV to +10 mV) applied in voltage clamp. Leak conductances were calculated in a data analysis program (Igor Pro) by linear regression to the slope of the essentially linear region of the membrane I-V curve (−100 mV to −65 mV). Cell capacitance (Cm) was determined from the integral of the transient capacitance current (IC, leak subtracted) evoked by a 15-ms hyperpolarizing voltage-step command applied within −10 mV of resting potential, using ∫ ICdt = −Qm at each command potential (Vm). Cm was determined from the slope of the plot of Qm vs. ΔVm for the series of step commands. Series resistance (RS) was calculated from the decay-time constant of IC, and compensated online by ≥80%. Neurons failing to meet the criterion Rm >10 RS necessary to achieve space clamp were excluded from voltage-clamp analysis. Furthermore, neurons with clear evidence of poor space clamp such as unclamped action potential currents during the slow voltage-clamp ramps were excluded from the analysis. Statistical significance was determined by a Student’s paired t-test on mean data. Data are presented as means ± SE unless otherwise indicated.
EK was calculated from the Nernst equation, EK = −RT/F ln[K]O/[K]I, which yielded values of EK = −72 mV, for the intracellular recording and extracellular solution K+ concentrations ([K]O = 8 mM, [K]I= 125 mM), and RT/F = 25.86 at 27°C (Hille, 2001). This value was compared to the membrane voltages at the intersection of the whole-cell I-V ramps for control and experimental (acid or halothane) conditions to assess if the equilibrium potential for the channel affected was consistent with EK.
The GHK equation for simple electro-diffusion of K+ may be written as: IK = PK (F 2Vm/RT)(([KI] – [KO] exp(−FV/RT))/(1 – exp(-FV/RT)) (Hille, 2001), where PK is the membrane permeability to K+. Since the constant that relates PK to K+ channel conductance is not known, PK was treated as a constant of proportionality. Substituting terms Vm = −110 mV to 10 mV, [K]I = 125 mM, [K]O = 8 mM, F/RT @ 27°C = 0.0385 mV-1 (Hille, 2001), yields the GHK equation as a proportionality between IK and Vm: IK Vm(17 exp(−0.0385Vm)/(1 – exp(−0.0385Vm); this proportionality was then graphed over the voltage range −110 to 10 mV and fit to the I-V curve for leak current by scaling IK.
For single-cell (sc) RT-PCR experiments, at the end of the whole-cell recording session, the cytoplasm was aspirated as completely as possible into the patch pipette under visual control and then immediately expelled into a thin-walled PCR tube containing reverse transcription reagents (Invitrogen Life Technologies, Carlsbad, CA). First strand cDNA was synthesized for 1.5h at 50°C in a mixture of MgCl (2 μl, 25mM), dNTPs (1 μl, 10 mM), BSA (0.7 μl, 143ng/μl), random hexamers (1 μl, 50 ng/μl), oligodT (0.7 μl, 0.5 μg/μl), RNasin (1.2 μl, 40 u/μl), DTT (1 μl, 0.1 M) and SuperScriptIII RT (1 μl, 200 u/μl). The entire reaction was either immediately used as template for multiplex PCR or frozen at −80°C until assayed.
Following reverse transcription, the cDNAs for TASK-1, and/or TASK-3 were amplified simultaneously with a multiplex PCR procedure using the following set of primers (from 5 prime to 3 prime): TASK-1 (Genbank accession # AFO31384) sense, CAC CGT CAT CAC CAC AAT CG (position 367 – 386), antisense, TGC TCT GCA TCA CGC TTC TC (position 882-863); TASK 3 (Genbank accession # NM053405) sense, ATG AAG CGG CAG AAT GTG CG (position 91-110), antisense, AGA AGA TCT TCA TCG GTA TT (position 854 – 835). The first multiplex PCR was performed as hot start in a final volume of 50 μl containing 12 μl reverse transcription reaction, 20-50 pmol of each primer, 0.2 mM dNTPs, 10 X High Fidelity PCR buffer with 2 mM MgCl2 and 5 U of Platinum Taq High Fidelity DNA polymerase (Invitrogen Life Technologies). The reaction mixtures were heated to 94°C for 2 min., 30 cycles (94°C, 30 sec.; 55°C, 30 sec.; 68°C, 1 min.) of PCR followed by a final elongation period of 10 min. at 68°C. The second round of PCR amplification was performed as individual reactions with individual primers, utilizing 1 μl of the first PCR reaction product under similar conditions with the following modifications: 50 pmole of each primer pair and 25 thermal cycles. 10 μl aliquots of PCR products were separated and visualized in an ethidium bromide-stained agarose gel (2%) by electrophoresis. The expected sizes of PCR-generated fragments were: TASK-1 (515 bp) and TASK-3 (763 bp).
To ensure that the PCR signal arose from the cytoplasm of the recorded cell, in each experiment we performed ‘mock harvests’ whereby a pipette was introduced into the slice but no cell contents extracted, and RT-PCR assays were run on harvested pipette solution as described above as negative controls from each brain slice. In all scRT-PCR assays 100 pg total rat brain RNA (Ambion, Austin, TX) was also run as RT template to serve as a positive control.
To theoretically examine and gain insight into regulation of intrinsic bursting and network oscillations of pre-BötC neurons by modulation of TASK-like leak conductances, we used our previous neuron models consisting of a single somal compartment incorporating a fast-activating, slowly inactivating persistent Na+ conductance (gNaP) and a K+-dominated ohmic leak conductance (gLeak) for the two major neuronal subthreshold currents as measured here and elsewhere (Koizumi and Smith, 2008), as well as Hodgkin-Huxley-like transient Na+ current and delayed-rectifier-like K+ current for action potential generation, as previously described in detail (Model 1) (Butera et al., 1999a; Del Negro et al., 2001). The pre-BötC excitatory network was modeled by 50 synaptically-coupled (Butera et al., 1999b) neurons with fast glutamatergic (AMPA)-like synaptic currents, and heterogeneous parameter values (below) that produced a mixture of cells with intrinsic and non-intrinsic bursting properties when synaptic conductance was set to zero (synaptically uncoupled), which is consistent with experimental observations that only a fraction of pre-BötC neurons exhibit intrinsic bursting properties when synaptic transmission is blocked (Koshiya and Smith, 1999; Purvis et al., 2007; Koizumi and Smith, 2008). Except for NaP steady-state activation properties, neuron capacitance values, and EK, all other Model 1 current parameters as well as parameters for phasic excitatory synaptic currents were identical to those specified previously (Butera et al., 1999a, 1999b). Steady-state activation properties for NaP used were based on Boltzmann function data obtained in our previous study (Koizumi et al., 2008) (V1/2max = −47 mV, k = 5.0); similarly data-based Cm (28 nS), and EK (−72 mV) values as calculated from the intra- and extracellular K+ concentrations under the present recording conditions, were used. The networks also incorporated a small constant background tonic post-synaptic excitatory conductance as previously described (Butera et al., 1999b), which was set at 0.1 nS. All simulations used all-to-all synaptic coupling for the 50 cells, the smallest population that preserves the dynamics observed for populations an order of magnitude larger (Butera et al., 1999b; Purvis et al., 2007). To incorporate parameter heterogeneity, neuronal gNaP, gLeak, and excitatory post-synaptic conductance values were randomly assigned within the network population from normal distributions with ± 30% SD for each parameter to mimic our experimental data (Purvis et al., 2007). Total neuronal leak conductance (gLeak) was partitioned into a dominant K+ component (gLeakK) and a small fixed cationic leak component as previously described (Del Negro et al., 2001; Koizumi and Smith, 2008). Numerical methods were identical to those described previously (Butera et al., 1999b), and simulations were run with Berkeley Madonna software. The initial 20 s of simulated time (typically 90 s total) was discarded. Network activity was displayed and analyzed from running histograms (adjustable bin size: 10-100 ms) of spike times computed and averaged across the population. Raster plots of neuron spiking (Butera et al., 1999b; Purvis et al., 2007) were used to assess neuronal burst synchronization within the network and stability of the network rhythm.
To determine if pre-BötC inspiratory neurons have TASK, we first tested functionally identified pre-BötC inspiratory neurons in isolated rhythmically-active in vitro neonatal rat slice preparations for the four electrophysiological properties of TASK channels: selectivity for K+, whole-cell I-V relations described by constant field theory, channel closure to extracellular acid, and channel opening to halothane.
We labeled and imaged rhythmically active pre-BötC inspiratory neurons in the slices with Ca2+-sensitive dye (CaG, Fig. 1A), allowing functional identification of cells for targeted whole-cell patch-clamp recording. All neurons analyzed (n = 78) exhibited spike discharge synchronized with the rhythmic motoneuronal population activity recorded from hypoglossal (XII) nerve roots (Fig. 1B), which was used to monitor inspiratory network activity in the slices (Koshiya and Smith, 1999; Koizumi and Smith, 2008). To functionally isolate the cells for voltage-clamp analysis of membrane currents, we blocked synaptic transmission by either bath-applied Cd2+ (200 μM) or the non-NMDA glutamate receptor antagonist CNQX (20 μM), which eliminated rhythmic excitatory synaptic drive currents (Koshiya and Smith, 1999). These inspiratory neurons had two distinct electrophysiological profiles: neurons exhibited either intrinsic voltage-dependent oscillatory bursting (n = 47), or only tonic spiking (n = 31 non-intrinsic bursters), when the baseline potential was depolarized after blocking excitatory synaptic transmission, as we have previously described (Koshiya and Smith, 1999; Del Negro et al., 2002). The intrinsic bursters were also revealed by ectopic bursting under current clamp before blocking synaptic transmission (Fig. 1C). For both types of cells, slow voltage-clamp ramps (30mV/s, range: −110 to +10 mV) revealed that all neurons exhibited N-shaped I-V relations that could be decomposed into two primary subthreshold conductances: an ohmic-like conductance, evident by the essentially linear region of the I-V curve below −65 mV (with little if any rectification at hyperpolarized voltages), and a voltage-activated, TTX-sensitive, inward persistent Na+ current (Del Negro et al., 2002; Koizumi and Smith, 2008) generating the negative slope region in the ~−60 mV to −40 mV membrane voltage range. Leak conductance (gLeak) was determined by linear regression to the slope of the passive region (−110 to −65 mV) of the I-V relation (Fig. 1D). Under control conditions, the total leak current in all neurons examined had a reversal potential ELeak (0 current intercept of regression line) between −70 and −60 mV (mean ELeak = −68 ± 3.4 mV), similar to the potential previously determined for ELeak (Koizumi and Smith, 2008), which was at a slightly more depolarized membrane voltage that the calculated K+ equilibrium potential (EK), indicating as we found previously that gLeak was K+-dominated, with a small non-K+ cationic conductance component. We have suggested that the latter arises from a relatively small, open non-selective cationic conductance (NALCN-like, Lu et al., 2007) with reversal potential between -10 and 0 mV (Koizumi and Smith, 2008; Ptak et al., 2009) and accounting for ~10% – 15% of gLeak under basal conditions.
We measured changes in gLeak in response to acid and/or halothane in functionally identified pre-BötC inspiratory neurons to test for contributions of a TASK-like K+ conductance component of gLeak. Acidification of the slice bathing solution (pH = 6.8) decreased the slope of the I-V relation in the linear region dominated by gLeak (Fig. 2A) (n = 6 non-intrinsically bursting inspiratory neurons in this series). The mean gLeak decreased by 1.0 ± 0.4 nS or 24% from the control average conductance value of 3.9 ± 0.8 nS (p < 0.0001) as computed by linear regression (average 95% confidence interval of 1.6% for the linear fit). The I-V relation of the leak conductance and change in gLeak by acid was obtained by subtracting the I-V curves and slopes before and after acid. The current had a equilibrium potential (see ELeakK in Fig. 2A) close to the calculated EK for the intracellular-extracellular solution K+ concentrations employed (−73.9 ± 3.2 mV vs. −72 mV calculated, see Methods). The small (~2 mV) deviation of the experimentally determined equilibrium potential may be attributable to K+ buffering in slices (Chen and Nicholson, 2000), with the [K+]O surrounding the neurons recorded reduced from 8 mM (bath solution) to ~7mM by buffering.
Halothane (1.0% – 2.0% in solution) (Fig. 2B) increased gLeak (n = 8 inspiratory neurons, with 2 intrinsic bursters) by 3.1 ± 1.5 nS or 66% above control values of 4.68 ± 2.7 nS (p < 0.0003) for this group of neurons (average increase of gLeak of 84.0 % and 56.2 % for non-intrinsic and intrinsic bursters, respectively). This halothane-sensitive leak current also had a equilibrium potential (−73.1 ± 2.8 mV) close to the calculated EK and the equilibrium potential was not significantly different (p >0.05) from that found for the current affected by acid (above).
We also tested for interactions between acid and halothane (n = 6 inspiratory neurons, with 2 intrinsic bursters and 4 non-intrinsic bursters in this group). In all cases bath-applied acidic aCSF (pH 6.8) following halothane reversed the increase of gLeak by halothane (Fig. 2C, data from a representative intrinsic burster shown), which is characteristic of TASK channels (e.g. Bayliss et al., 2003). There were no obvious differences in the responses of intrinsic bursters and non-intrinsic bursters to halothane and acid, so the data for these two cell types were pooled. The mean gLeak with halothane (2%) increased in this group of neurons by 54% (from 2.9 ± 0.9 nS control values to 4.45 ± 1.47 nS, p < 0.001), and gLeak returned to 3.03 ± 1.04 nS with halothane + acid (pH 6.8), which was close to the control values.
To further characterize the I-V relations of gLeak, we bath-applied solutions with blockers of voltage-activated Nav + (with 1 μM TTX), Ca2+ (with 200 μM Cd2+) and Kv + channels (with 10 mM extracellular TEA) as well as non-selective cationic current Ih (with ZD7288, 100 μM) and other potential K+ channel contributors to Leak such as inwardly rectifying K+ conductances (Kir, blocked with 200 μM Ba2+). Sirois et al. (2002) found a small effect of halothane in neurons attributable to Ih when they applied the Ih channel blocker ZD7288, and some Kir’s are acid sensitive (e.g. Zhu et al., 1999; Xu et al., 2000). The I-V relations obtained in the presence of these blockers was linear at hyperpolarized voltages and exhibited slight outward rectification at depolarized voltages (Fig. 3). Non-intrinsic bursters (Fig. 3A) and intrinsic bursters (Fig. 3B) had similar I-V relations under these conditions, and responses of these two cell types to acid or halothane were also similar so data were again pooled for the groups exposed to acid or halothane. The mean gLeak in these neurons again decreased in response to acid on average by 22.6% and 25.6% at pH = 7.0 (n = 2, with 1 intrinsic burster) and 6.8 (n = 3, with 1 intrinsic burster), respectively, from control values in the presence of blockers (Fig. 3A). The average gLeak increased by 59.8% from control (n = 4, with 2 intrinsic bursters) in response to halothane (2%) (Fig. 3B). I-V relations of the affected conductance obtained by I-V curve subtraction in all cases conformed to the shape of the I-V curve predicted from GHK constant field theory (examples shown in Fig. 3A,B) for K+ electro-diffusion through an open K+-selective channel, and the mean reversal potentials (ELeakK) for the acid and halothane affected conductance were not different (pooled values of −74.2 ± 3.4 mV for ELeakK, n = 9) and were close to the calculated EK.
To further validate our approach, we also measured I-V relations and the change in gLeak of inspiratory XII motoneurons (Koizumi et al., 2008) in response to bath-applied halothane solution (2%) in the slice preparations. Consistent with previous results that have demonstrated TASK channels in XII motoneurons (Sirois et al., 2000; Sirois et al., 2002), we found that halothane increased gLeak of inspiratory XII motoneurons by an average of 57% (from control gLeak values of 9.64 ± 1.75 nS to 15.05 ± 2.72 nS, n = 11 inspiratory motoneurons) (I-V data not shown).
TASK mRNA has been shown to be present by in situ hybridization in adult rat pre-BötC neurons (Washburn et al., 2003) reputed to be respiratory neurons via their co-expression of neurokinin-1 receptors (Gray et al., 1999), which is not an exclusive marker for pre-BötC respiratory neurons (Gray et al. 2001; Pagliardini et al., 2005). The pre-BötC region has a heterogeneous neuronal composition with many non-respiratory neurons, requiring electrophysiological identification of respiratory neurons. We therefore assayed for TASK channel mRNA in cytoplasm harvested during whole-cell recording from identified pre-BötC inspiratory neurons including cells with intrinsic bursting properties (n = 14 inspiratory neurons total, with 4 intrinsic bursters and 10 non-intrinsically bursting neurons assayed). Cytoplasm was aspirated into the pipette and assays by scRT-PCR were performed for TASK-1 mRNA in one group of cells (n = 9), or for both TASK-1 and TASK-3 mRNA in another group (n = 5). TASK-1 mRNA was found in 6 of the 9 pre-BötC inspiratory neurons assayed in the first group (with 2 of 3 intrinsic bursters and 4 of 6 non-intrinsic bursters tested expressing TASK-1 mRNA). TASK-1 and TASK-3 mRNA were found together in 2 of 5 cells assayed in the other group of inspiratory neurons (1 of 2 intrinsic bursters and 1 of 3 non-intrinsic bursters tested in this group expressed both TASK-1 and TASK-3 mRNA) (Fig. 4). For any TASK-expressing inspiratory neuron assayed, no TASK-1 or TASK-3 signals were detected in negative controls from “mock harvests” in the slice (see Materials and Methods).
Does the TASK-like leak conductance regulate intrinsic rhythmic bursting behavior of pre-BötC neurons? We predict that acid, by decreasing K+ leak conductance of pre-BötC bursters causes depolarization, resulting in an increase in intrinsic, voltage-dependent bursting frequency (Butera et al., 1999a; Del Negro et al., 2001; modeling results below). To test this prediction, inspiratory neurons were isolated from synaptic input by bath-applied Cd2+ (200 μM) to identify NaP-dependent intrinsic bursting (Koizumi and Smith, 2008), and bursting behavior of identified neurons was recorded in whole-cell current-clamp. For these experiments we used blind whole-cell patch-clamping procedures (Koizumi et al., 2008) to include in the sample neurons deeper in the slice than could be resolved by our optical imaging approaches. For voltage-clamp measurements Na+ currents were also blocked with TTX (1μM). In correspondence with the overall population of inspiratory neurons as described above, with exposure of the slice to acidic (pH 6.8) aCSF, gLeak of all intrinsic bursters tested (n = 19) decreased in this group of inspiratory cells from a mean value of 2.6 ± 0.7 nS at control pH 7.4 to 2.1 ± 0.6 nS (p = 0.0001) as determined from the slope of the linear fit to the ramp I-V curves at hyperpolarized voltages (<-65 mV). The average reduction in gLeak (20% from control values) with acidification in this group of intrinsic bursters was similar to that obtained for the group of intrinsic bursters and non-intrinsic bursters (24% – 26% reduction in average gLeak, pooled data) described above that were recorded at more superficial locations in the slices. Furthermore, in another group of intrinsic burster neurons tested (n = 16) under current clamp recording, consistent with the hypothesis that TASK-like leak conductance regulates cellular rhythmic bursting, decreasing aCSF pH from pH 7.4 to pH 6.8 depolarized the baseline membrane potential (from −49.5 ± 5.5 mV to −44.0 ± 6.0 mV, p = 0.0001) (Fig. 5), and increased the averaged maximum neuronal bursting frequency (from 0.1 ± 0.03 Hz to 0.2 ± 0.09 Hz, p = 0.00039).
Based on our results that TASK-like leak regulates rhythmogenesis at the cellular level, we analyzed modulation of inspiratory rhythm by acid and halothane at the network level, monitored by XII motor population discharge. Halothane-containing aCSF applied to the slice monotonically decreased steady-state inspiratory discharge frequency and terminated rhythmic network activity, in a concentration-dependent manner, and terminated rhythmic network activity (n = 22 slices) (Fig. 6B,C, E). Acidic aCSF applied to the slice increased XII discharge frequency (n = 11, 178 ± 44% of control, p < 0.0003 at pH 6.8) (Fig. 6A,E), and diagnostic of involvement of TASK channels in modulation of the rhythm, reactivated rhythmic network activity in the presence of halothane (n = 7) (Fig. 6C, D, E). The effect of acid (pH 6.8) dominated over the effect of halothane when halothane and acid were applied together: the acid induced increase of XII discharge frequency (174 ± 74% of control, p < 0.04, n = 7) in the presence of halothane, was nearly as large as the frequency increase by acid alone (Fig. 6E).
To establish whether modulation of network rhythm by acid and halothane involved perturbations of neuronal excitability at the level of the pre-BötC network, acidic or halothane-containing aCSF was bilaterally microinfused directly into the core of the imaged pre-BötC (see Fig. 1, n = 5 slices). This circumvented the possibility of network-wide modulation of rhythm by neurons outside of the pre-BötC in the slice that may be acid/halothane sensitive and can modulate pre-BötC neuron excitability. There is TASK in hypoglossal motoneurons (e.g. Talley et al., 2000), and also in raphé nuclei (Washburn et al., 2002), which have chemosensory properties (Richerson, 2004; Mulkey et al., 2007) and excitatory serotonergic neuronal projections to pre-BötC and hypoglossal respiratory neurons (Ptak et al., 2009). Microinfusion of acidic aCSF (pH 7.2, 7.0, 6.8, 6.0) bilaterally into the core of the pre-BötC increased the frequency of XII inspiratory discharge (Fig. 7A,B,C). The onset of elevation of burst discharge frequency was faster than when the slice was superfused with acidic solution. Quantitatively, the acid-induced increase in discharge frequency was dose-dependent (Fig. 7C) with a maximal mean increase of 225% above control at pH 6.0. The calculated Hill slope of the pH vs. frequency relation was 0.84. Bilateral microinfusion of halothane-containing aCSF (2% in pipette solution, n = 4) progressively decreased XII burst frequency and terminated rhythm generation, whereas bath-applied acidic aCSF (pH 6.8, n = 5) reversed the halothane induced slowing of network rhythm (Fig. 7D,E).
To further investigate the link between modulation of TASK-like leak conductance at the cellular level and modulation of rhythmic bursting activity at cellular and network levels, we analyzed control of rhythm by a K+ leak conductance in single neuron models of intrinsically bursting pre-BötC cells (Butera et al., 1999a; Purvis et al., 2007) and a rhythmic excitatory network model of the pre-BötC (Butera et al., 1999b; Purvis et al. 2007), consisting of a heterogeneous mixture of 50 intrinsically bursting and non-intrinsically bursting model neurons (Butera et al, 1999b; Purvis et al. 2007; Koizumi and Smith, 2008). Neurons in these models had voltage-clamp ramp I-V relations and leak conductances similar to those measured experimentally here and elsewhere (Purvis et al., 2007; Koizumi and Smith, 2008). The total neuronal leak conductance, gLeak, was partitioned into a K+ conductance component (gLeakK) and a smaller non-K+ mixed cationic conductance component (see Modeling methods), which we estimated is ~10% of gLeak under basal condition. We analyzed modulation of rhythmic cellular/network activity as the neuronal K+ component was varied over a range of values predicted from the measured gLeak in whole-cell voltage-clamp recording and changes in gLeakK with acidic and halothane conditions. Since the voltage-activated persistent Na+ current (NaP) dynamically interacts in the neuronal model with the leak current (Koizumi and Smith, 2008), simulations of the models were run over the normal range of single neuron NaP conductance (gNaP) measured in pre-BötC inspiratory neurons in neonatal rat slices in vitro (Purvis et al., 2007; Koizumi and Smith, 2008) to examine the modulatory role of gLeakK for a range of possible cellular/network initial conditions.
We first analyzed the behavior of a model intrinsically bursting pre-BötC neuron as the single-cell gLeakK was varied (Fig. 8). In the parameter space covering the experimentally measured values of gNaP, values of gLeak (here and Purvis et al. 2007), and estimated values of gLeakK, the single-neuron model (Butera et al., 1999a) was well behaved in that for a given gNaP, neuronal bursting frequency decreased monotonically to 0 Hz with increasing gLeakK (Fig. 8A,B), and the range of burst frequencies (0 – 0.35 Hz) covered the experimentally observed range. The single neuron model was bounded by gLeakK = 2.0 nS, below which the model neuron spikes tonically at a given gNaP, and by gNaP = 2.0 nS, below which the model neuron is silent at a given gLeakK. The estimated mean value of gLeakK for pre-BötC intrinsic bursters for acidic conditions (~2.0 nS at pH 6.8), when plotted on the gNaP isopleths of 2.4 nS or 3.6 nS, which bound most of the measured range for gNaP in pre-BötC intrinsic bursters (Purvis et al., 2007), yielded a range of burst frequencies similar to that recorded here from intrinsic bursters under acidic conditions (0.2 – 0.3 Hz). For simulated halothane conditions (estimated gLeakK = ~6.0 – 7.0 nS), the model is silent (not intrinsically bursting) for any value of gNaP. Thus modulation of a TASK-like gLeakK, mimicking experimentally observed average ranges of gLeakK obtained with acid and halothane, yielded in the model a dynamic range of burst frequencies typical of that recorded from single intrinsically bursting pre-BötC neurons.
For network simulations, we distributed estimated values of neuronal gLeakK to yield a mean population value (GLeakK) with SD ± 30% for a 50-neuron population to model the heterogeneous population of pre-BötC neurons consisting of a mixture of intrinsic and non-intrinsically bursting inspiratory neurons. The statistical distribution of gLeak values conformed with that found experimentally here and previously (Purvis et al., 2007) for a mixed population of pre-BötC inspiratory cells. Network simulations (Koizumi and Smith, 2008), in which GLeakK was varied over the range corresponding to mean values of gLeakK obtained for acidic and halothane conditions, exhibited a range of burst frequencies similar to that observed experimentally (from data summarized in Fig. 6, and network frequencies shown in Fig. 7), zero to ~0.5 Hz (Fig. 9A,B). For a given value of population mean NaP conductance (GNaP, also distributed over the population with ± 30% SD, see Methods), the network burst frequency decreased monotonically to zero with increasing GLeakK. The estimated value of GLeakK of 3.5 nS for the general population of inspiratory neurons (intrinsic bursters and non-intrinsic bursters) under control conditions, coupled with the GNaP value of 2.4 nS measured previously (Purvis et al., 2007), yielded in the model network simulations burst frequencies of ~0.15 Hz, similar to bursting frequencies recorded from the slice network under control conditions. For the range of GLeakK values (2.5 – 3.0 nS) estimated for acidic conditions for the general population, with a GNaP of 2.4 nS, a network bursting frequency range of ~0.3 – 0.5 Hz obtained in the model simulations, covering the frequency range observed experimentally during slice perfusion or pre-BötC microinfusion of acidic aCSF. Over the estimated range of GLeakK with network exposure to halothane (6.0 – 7.0 nS), network burst frequency is zero, consistent with our observations for the rhythmic slice during halothane superfusion or pre-BötC microinfusion. Thus our network simulation results suggest that modulation of a cellular TASK-like K+ leak conductance can be directly expressed as modulatory effects on rhythm at the network level.
We obtained evidence for TASK channels within inspiratory neurons of the pre-BötC by scRT-PCR and established electrophysiologically that TASK-like channels are functional in pre-BötC cells. Our cellular-level voltage-clamp measurements for both intrinsic and non-intrinsically bursting pre-BötC inspiratory neurons satisfied the four diagnostic properties of TASK channels differentiating these channels from all other known channels: selectivity for K+, I-V relations described by constant field theory, channel closure to extracellular acid, and channel opening to halothane. Our single-cell recordings furthermore showed that pre-BötC inspiratory neurons are depolarized and intrinsically bursting neurons accordingly exhibited increased bursting frequencies with exposure to acid as predicted for contributions of TASK to gLeak. Finally, the inspiratory bursting frequency of the pre-BötC network is modulated by acid and halothane, consistent with the cellular-level changes in gLeak measured and also predicted by our computational models with modulation by the K+ component of leak conductance.
Pre-BötC neurons exhibit a classic leak conductance at membrane voltages below those at which non-linear voltage-dependent conductances activate (here and Koizumi and Smith, 2008). Ramp I-V relations were essentially linear over this subthreshold voltage range, and after blocking voltage-activated conductances, the I-V relations over a wider voltage range exhibited weak outward rectification. We tested for the signature dual responses of TASK to acid and halothane (Lesage and Lazdunski, 2000; Talley and Bayliss, 2002) and demonstrated reduced gLeak with exposure to acid and an augmented conductance by halothane that could be completely reversed by acid. Furthermore, I-V relations for the acid- and halothane-associated conductances had reversal potentials near Ek and conformed to predictions from the GHK constant field equation for K+ channels. All of these characteristics are consistent with properties of TASK channels. We note however that while these biophysical and pharmacological criteria to identify TASK channels are standard with proven reliability, many of these same criteria have been used to implicate functional involvement of TASK channels in some neurons, particularly for glucose sensing in orexin neurons (Burdakov et al., 2006), but this conclusion was subsequently proven incorrect (Guyon et al., 2009; Gozalez et al., 2009). Thus definitive molecular identification of TASK channels in pre-BötC neurons based on the above criteria remains tentative.
Do K+ channels other than TASK-1 and TASK-3 contribute to the modulation of leak conductance by acid? G-protein-coupled inwardly rectifying K+ channels (Kir) can modulate inspiratory rhythm generation in vitro (Johnson et al. 1996), and at least three types of Kir channels, Kir 2.3 (Zhu et al., 1999), Kir 4.1, and Kir 4.1-5.1 (Xu et al., 2000), are acid sensitive. Kir 4.1 conductance decreases in response to acid with a pK of 6.2 matching that of TASK-3, and Kir 4.1-5.1 conductance decreases in response to acid with a pK of 7.4 matching TASK-1, while the pK for Kir 2.3 is intermediate at 6.8. However, the sensitivity of these Kir’s is to intracellular, not extracellular acid. The pH of our whole-cell recording pipette solution was strongly buffered at 7.3 – 7.4 with HEPES. Furthermore, since the acid-modulated leak I-V relations in our measurements were outwardly and not inwardly rectifying, and conductance changes obtained were unaffected by Kir blockers, Kir likely did not mediate acid-induced changes in gLeakK. Channels linked to putative chemosensory purinergic (P2) receptors are also unlikely to be involved because these receptors do not mediate chemosensory responses of pre-BötC cells (Lorier et al., 2007; Funk et al., 2008).
In our whole-cell recordings a non-rectifying leak conductance persisted even at an acidification of pH 6.5 (not shown). Since TASK-1 channels are almost entirely closed at pH 6.5 (Berg et al., 2004), this residual conductance is not from TASK-1. The pK for TASK-3 is ~6.5 (Berg et al., 2004) so the residual conductance could be due to TASK-3. This inference is supported by our preliminary results from a small number of slices (n = 3) showing that isoflurane (0.5%), which specifically blocks TASK-3 (Berg et al., 2004), reduces network bursting frequency to nearly zero. Furthermore we found that the pH range over which microinfusion of acid into the pre-BötC monotonically increased inspiratory bursting frequency extended to pH 6.0.
Our experimental analyses show that halothane down-regulated, and extracellular acid augmented, network-level inspiratory bursting frequency when these TASK modulators were either bath applied or directly microinfused bilaterally into the pre-BötC. Furthermore, our computational results suggest how modulation of a TASK-like K+ component of leak conductance, distributed over a model heterogenous excitatory network of neurons with subthreshold I-V relations dominated by Leak and NaP (here and Koizumi and Smith, 2008), can account for our experimental observations. Reducing or augmenting GLeakK, respectively, causes neuronal depolarization or hyperpolarization within the network with concomitant increases or deceases in population-wide bursting frequency over a dynamic range similar to that observed experimentally. Taken together with our cellular-level analysis, the experimental and computational results suggest that modulation of a TASK-like K+ leak conductance can be directly expressed as modulatory effects on inspiratory rhythmic activity at the network level. While our results with local microinfusion of halothane and acid into the pre-BötC are consistent with predictions based on our cellular measurements and model simulations, we note that we cannot exclude the possibility that in some experiments the suppression of network activity by local halothane and its subsequent reversal by reduced pH (Fig. 7D,E) could involve different channels in different neurons, especially since the reversal of local halothane effects were obtained with bath acidification. At present, however, we favor the most parsimonious explanation that the perturbations of network inspiratory activity observed are due to TASK channel modulation in pre-BötC neurons.
Since TASK channels are instantly activating, non-inactivating, outwardly rectifying, and are selective for K+, most investigators in the K2P channel field immediately inferred that TASK provides a K+ component of neuronal leak conductance. Butera et al. (1999a,b) originally proposed that the ohmic-like leak current of neurons comprising the pre-BötC inspiratory rhythm generator is K+-dominated and provides a basic mechanism for modulation of rhythm generation at cellular and network levels. Meuth et al. (2003) provided the first experimental evidence that TASK channels are a component of leak currents controlling activity of a neural rhythm generator. Here we present evidence that TASK channels provide a K+ leak conductance-based mechanism for chemosensory-related modulatory control of pre-BötC rhythm generation.
A number of neurotransmitters with G-protein-coupled receptors close TASK channels (Bayliss et al., 2003; Mathie, 2007). In recombinant systems, TASK closes in response to TRH (Talley and Bayliss, 2002), angiotensin II (Czirjak et al., 2000), and muscarinic M1 receptor agonists (Czirjak et al., 2001). Other neurotransmitters, including substance P (SP), serotonin (5-HT), norepinephrine, and glutamate (acting via metabotropic glutamate receptors) also close a leak conductance that has TASK-like acid and halothane sensitivity (Talley et al., 2000). Thus as proposed for other neurons (Bayliss et al., 2003; Mathie, 2007), TASK channels may constitute a convergent target for neuromodulatory control of pre-BötC rhythm generation. SP and 5-HT have been shown to augment pre-BötC cellular and network bursting by reducing a TASK-like K+ component of leak conductance in pre-BötC inspiratory neurons (Koizumi and Smith, 2008; Ptak et al., 2009), although these neuromodulators act simultaneously via other cationic components of leak such as a NALCN-like component (Ptak et al., 2009) that also cause neuronal excitation. Thus there appears to be duality in modulatory control involving several channel entities comprising discrete leak conductance components of which TASK represents one important set of K+ background channels.
Recent studies with TASK-1 and TASK-3 knockout mice (Mulkey et al., 2007; Trapp et al., 2008) have not demonstrated abnormal baseline breathing in vivo, although TASK-1 knockouts show abnormal ventilatory responses to hypoxia and moderate hypercapnia, attributed to peripheral (Trapp et al., 2008) but not some critical central brainstem chemoreceptive cells (Mulkey et al., 2007). TASK-1 should normally be open at physiological pH, but the observations of normal baseline breathing in the knockout mice may imply that: (1) other K+ background channels are also major components of the K+-dominated leak of pre-BötC neurons; (2) other K+ channel components are up-regulated in these knockouts, including in cells involved in chemoreception that may exhibit compensatory changes is spontaneous firing behavior (Trapp et al., 2008) to regulate activity of the respiratory network by afferent input to the pre-BötC and other network components; and (3) other leak channels such as NALCN that normally co-mediate modulatory actions of neuromodulators such as SP and 5-HT, which critically control pre-BötC network excitability (Ptak et al., 2009), are sufficient for neuromodulatory control. K+ channel candidates that may be other normal components of leak or are up-regulated include other K2P channels such as TWIK (Lesage et al., 1996), TREK (Fink et al., 1996), and TRAAK (Fink et al., 1998), or a yet unknown background K+ channel(s).
In summary, we have presented evidence that a component of the K+-dominated leak conductance of pre-BötC neurons is mediated by TASK-like channels. Accordingly, TASK may constitute a convergent target for modulatory control of pre-BötC rhythm generation, including by regulatory signals associated with CO2/H+ as well as neuromodulators that critically control pre-BötC rhythmic activity.
The authors thank Murtaza Mogri for scripting modeling simulations. This research was supported by the Intramural Research Program of the NIH, NINDS.