Ischemic preconditioning is an important intrinsic mechanism for neuroprotection. Preconditioning can also be achieved by exposure of neurons to K+ channel-opening drugs that act on adenosine triphosphate-sensitive K+ (K(ATP)) channels. However, these agents do not readily cross the blood-brain barrier. Inhalational anesthetics which easily partition into brain have been shown to precondition various tissues. Here, the authors explore the neuronal preconditioning effect of modern inhalational anesthetics and investigate their effects on K(ATP) channels.
Neuronal-glial cocultures were exposed to inhalational anesthetics in a preconditioning paradigm, followed by oxygen-glucose deprivation. Increased cell survival due to preconditioning was quantified with the 3-(4,5-dimethyl-2-thiazolyl)-2,5-diphenyl-2H-tetrazolium bromide reduction test. Recombinant plasmalemmal K(ATP) channels of the main neuronal type (Kir6.2/SUR1) were expressed in HEK293 cells, and the effects of anesthetics were evaluated in whole cell patch clamp recordings.
Both sevoflurane and the noble gas xenon preconditioned neurons at clinically used concentrations. The effect of sevoflurane was independent of K(ATP) channel activation, whereas the effect of xenon required the opening of plasmalemmal K(ATP) channels. Recombinant K(ATP) channels were activated by xenon but inhibited by halogenated volatiles. Modulation of mitochondrial K-ATP channels did not affect the activity of K(ATP) channels, thus ruling out an indirect effect of volatiles via mitochondrial channels.
The preconditioning properties of halogenated volatiles cannot be explained by their effect on K(ATP) channels, whereas xenon preconditioning clearly involves the activation of these channels. Therefore, xenon might mimic the intrinsic mechanism of ischemic preconditioning most closely. This, together with its good safety profile, might suggest xenon as a viable neuroprotective agent in the clinical setting.
EARLY ischemic stroke after heart surgery has a high incidence and is associated with substantial disability and mortality rates.1–3Although volatile anesthetics have been found to initiate early phase ischemic tolerance in neurons, models of focal brain ischemia suggest that it can be expected to take 24 h for the preconditioning to develop its full effectiveness.4,5Therefore, cardiac surgical patients are likely to be exposed to the greatest risk of cerebral ischemic damage in a phase where they are least protected. Consequently, neuroprotective strategies should be implemented well in advance of surgery to allow pathways to become fully activated. This stratagem is possible with the use of pharmacologic preconditioning.
The concept of preconditioning describes the phenomenon that an organ achieves protection against potentially lethal insults through preexposure to harmful stimuli.6The term gained wide recognition in the late 1980s after the observation that brief episodes of reduced myocardial perfusion before the extended, harmful ischemic period, diminished tissue damage, and preserved cardiac function.7Subsequently, preconditioning was also found in other organs, such as brain and kidneys, and this boosted clinical and scientific interest in this phenomenon.
Although a large body of studies thus far failed to unravel the entire cellular signaling pathways that lead to preconditioning, it became clear that adenosine triphosphate–sensitive K+(KATP) channels can play a critical role in the process.6This view received further support from recent studies demonstrating that genetic ablation of the pore-forming subunit Kir6.2 of the plasmalemmal KATPchannel causes the loss of ischemic preconditioning of cardiac tissue8–10and the loss of neuroprotection against acute hypoxia.11Although these findings unequivocally demonstrated that the opening of plasmalemmal KATPchannels is beneficial for cell survival, several drawbacks limit the scope for clinical exploration. For example, currently there is no convincing evidence that established KATPchannel openers such as diazoxide readily cross the blood–brain barrier. This is different with anesthetics because penetration of the blood–brain barrier is one of the defining characteristics of this class of substances. Moreover, there is not only a vast amount of clinical experience in their safe use, but outcome parameters can also be directly monitored.
The noble gas xenon has been proposed as an alternative to classic anesthetics partly because of its suggested organ protective effects and its overall benign side effect profile.12However, its high production cost has so far stopped it from being used widely.13
A number of reports suggest that other inhalational anesthetics have preconditioning effects on cardiac tissues, and a few studies suggest they have neuroprotective properties, though there is no consensus about their mode of action.14–16
Those studies that explored the involvement of KATPchannels in anesthetic preconditioning in the brain have focused almost exclusively on the role of mitochondrial K-ATP (mito K-ATP) channels17,18; no study has ever examined the involvement of plasmalemmal KATPchannels in neuronal preconditioning induced by either of the newer inhalational anesthetics sevoflurane or xenon. Furthermore, the majority of studies have not investigated the effects of drugs directly on KATPcurrents but simply relied on the perceived specificity of the drugs used for channel subtypes.19
With the current study, we aim to clarify the role of KATPchannels in preconditioning induced by the inhalational anesthetics xenon and sevoflurane. We hypothesize that the opening of plasmalemmal ATP-sensitive K+channels rather than mito K-ATP channels is required for neuronal preconditioning by these drugs. We also postulate that to verify the preconditioning action of these drugs via KATPchannels, their direct stimulatory action on currents through these ion channels in a recombinant expression system must be evident.
Materials and Methods
Tissue culture neuronal–glial cell cocultures were prepared as described previously.20All procedures involving animals were performed in accordance with the Animals (Scientific Procedures) Act 1986 and approved by the Home Office, London, United Kingdom. In brief, brains from 1- to 2-day-old BALB/c mouse pups were removed from the skull and microdissected to obtain whole cerebral neocortices. After trypsination and resuspension, cells were plated at a density of 6.25 × 104cells/cm2on four-well plates (Nunc, Roskilde, Denmark). They were cultured in Eagle's minimum essential medium supplemented with 20 mm glucose, 26 mm NaHCO3, 10% fetal bovine serum, 10% heat-inactivated horse serum, Antibiotic-Antimycotic Solution (AAS; Gibco, Paisley, United Kingdom), 2 mm glutamine (Sigma, Poole, United Kingdom), and 10 ng/ml murine epidermal growth factor (Gibco). Glial cells reached confluence approximately 5 days after plating. Using a similar procedure, cortical neuronal cells were obtained from fetal BALB/c mice at 14–16 days of gestation and were plated at a density of 1.25 × 105cells/cm2onto the confluent monolayer of glial cells. Neuronal cells reached mature morphology within 10 days after plating, and cocultures were used for preconditioning experiments after a total of 15 ± 1 day. Cultures were assigned to one of the following protocols: preconditioning, oxygen–glucose deprivation (OGD) only, or naive control. Cultures in the preconditioning group were exposed to either 1 minimum alveolar concentration (MAC) xenon, 2 MAC sevoflurane, or 10 μm diazoxide for 2 h in the presence or absence of the KATPchannel inhibitor tolbutamide (0.1 mm) or the inhibitor of mito K-ATP channels 5-hydroxy-decanoic acid (5-HD, 0.5 mm).
Preconditioning was performed as described previously.21Anesthetic-enriched medium was obtained by bubbling xenon or sevoflurane for 15 min through experimental medium containing Eagle's minimal essential medium, 21.1 mm glucose, and 38 mm NaHCO3in a Drechsel bottle. Neuronal–glial cell cocultures were washed twice with HEPES-buffered solution (120 mm NaCl, 5.4 mm KCl, 0.8 mm MgCl2, 15 mm glucose, and 2.0 mm HEPES, titrated to pH 7.4 using 1 m NaOH) and then incubated with anesthetic-enriched medium or with experimental medium containing 10 μm diazoxide. Tolbutamide (0.1 mm) or 5-HD (0.5 mm) were added to some dishes as appropriate. Cocultures were then transferred to an airtight, temperature-controlled gas exposure chamber for 2 h. The gas composition in the chamber for the xenon experiments consisted of 20% O2, 5% CO2, and 75% xenon (approximately 1 MAC). The gas composition in the sevoflurane experiments was 20% O2, 5% CO2, 71.7% N2, and 3.3% sevoflurane (2 MAC). The atmosphere in the chamber for diazoxide preconditioning consisted of 20% O2, 5% CO2, and 75% N2. After 2 h, cultures were removed from the chamber, washed with HEPES-buffered solution, and finally incubated in culture medium until further use.
Cocultures of the OGD group underwent the same protocol as the cultures in the preconditioning group except that instead of being exposed to HEPES-buffered solution containing the preconditioning drugs, they were washed with HEPES-buffered solution only. Cultures of the naive control group received the same pattern of solution changes but were not exposed to the preconditioning drugs or OGD.
To model ischemic injury in the brain, neuronal cells were subjected to OGD.22Twenty-four hours after preconditioning, cultures were washed twice with HEPES-buffered solution and once with prewarmed OGD medium. OGD medium contained 116 mm NaCl, 5.4 mm KCl, 0.8 mm MgSO4, 1.0 mm NaH2PO4, 1.8 mm CaCl2, and 26 mm NaHCO3and was bubbled with 5% CO2and 95% N2in a Drechsel bottle at 37°C. Cultures were then placed into an airtight gas exposure chamber with an anaerobic environment consisting of 5% CO2and 95% N2at 37°C for 75 min. OGD was terminated by removing cultures from the chamber and changing the media back to the culture medium.
MTT Reduction Test
The 3-(4,5-dimethyl-2-thiazolyl)-2,5-diphenyl-2H-tetrazolium bromide (MTT) reduction test is a quantitative measurement of cellular metabolic activity and therefore widely used for the assessment of cellular viability and cell proliferation.23,24In the presence of active mitochondrial and cytosolic redox systems, the tetrazolium salts of MTT are reduced to intensely blue-colored formazans, which can be quantified in a spectrophotometer. The measured optical density corresponds directly to the viability of the cells in culture. Cell viability is stable between 6 and 24 h after OGD25; therefore, the MTT test was performed on the following day. Neuronal–glial cocultures were incubated for 2 h in 600 μl phosphate-buffered saline with 0.5 mg/ml MTT (Merck, Darmstadt, Germany) to allow uptake of MTT into the cells. After removing MTT from cultures, cells were dissolved and homogenized in 1 ml dimethyl sulfoxide (DMSO). Then, 0.3 ml of each sample was transferred to one well of a 96-well plate. The optical density (OD) was measured in triplicate at 570 nm in an MRX Microplate Reader (Dynex Technologies, Chantilly, VA).
The OD readings were then converted into normalized cell viability readings using equation 1:
where % Cviais cell viability expressed in percent, ODdrugis the optical density reading of preconditioned cells, ODcontrolis the optical density reading of untreated naive cells, and ODOGDis the optical density reading of nonpreconditioned cells, which were exposed to OGD only.
Recombinant KATPChannel Studies
HEK293 cells were maintained in growth medium (minimum essential medium enriched with 10 ml per 500 ml penicillin–streptomycin solution, 5 ml per 500 ml minimum essential medium nonessential amino acids, 50 ml per 500 ml fetal bovine serum, and 2 mm l-glutamine) in 5% CO2–95% O2in a humidified incubator at 37°C. When the cells were 80% confluent (after approximately 4 days), they were plated onto glass coverslips coated with poly-D-lysine (1 mg/ml), and after a 6-h resting period, transient transfection was performed using the calcium phosphate method.26Cells were transfected with pcDNA3 vectors containing the coding sequence of mouse Kir6.2 (Genbank D5058127,28), rat SUR1 (Genbank L4062429), and green fluorescent protein. Cells were then incubated at 3% CO2–97% O2for 6–8 h. Subsequently, cells were washed twice with phosphate-buffered saline and incubated in growth medium in 5% CO2–95% O2in a humidified incubator at 37°C for 24–96 h until use for electrophysiologic recordings.
Stock solutions of tolbutamide (50 mm), diazoxide (20 mm), and pinacidil (10 mm) were prepared in 100 mm NaOH. Solutions containing sevoflurane, isoflurane, or halothane were prepared as volume fractions of a saturated aqueous solution. The concentration of these saturated solutions was taken as 11.8, 15.3, and 17.5 mm, respectively.30Solutions for the xenon experiments were prepared by bubbling extracellular solution with pure gases (xenon, nitrogen, oxygen) at a rate of 30 ml/min for 20 min, producing saturated solutions for the individual gases.31The test solutions with fractional gas concentrations were then obtained by mixing adequate volumes of the individual solutions with maintaining 20% oxygen–saturated solution and the balance (80%) being made up by varying amounts of nitrogen- and xenon-saturated solutions. Immediately after mixing, these solutions were transferred to glass syringe barrels containing a polypropylene float.31All other drugs were added directly to the experimental solutions, which were prepared freshly each day. Xenon was obtained from Air Products (Basingstoke, United Kingdom), sevoflurane and isoflurane were obtained from Abbott (Queenborough, Kent, United Kingdom), and nitrogen and oxygen were obtained from BOC (Manchester, United Kingdom). All other chemicals were from Sigma (Poole, Dorset, United Kingdom).
For electrophysiologic recordings, a coverslip with transfected HEK cells was transferred into a recording chamber mounted under an upright microscope (Zeiss Axioskop 2FS; Carl Zeiss Ltd., Welwyn Garden City, United Kingdom) with epifluorescence. During the course of the experiment, cells were constantly superfused at 3–5 ml/min with extracellular solution of the following composition: 118 mm NaCl, 3 mm KCl, 1 mm MgCl2, 1.5 mm CaCl2, and 25 mm HEPES (pH adjusted to 7.4 with NaOH). Test drugs were added to this solution either directly or from stock solutions as described above. Only cells that were successfully transfected with green fluorescent protein as evident from green fluorescence (excitation: 395–440 nm, emission: 470–600 nm) were selected for electrophysiologic recordings.
Patch pipettes were pulled from thin-walled borosilicate glass (GC150TF; Harvard Apparatus, Edenbridge, Kent, United Kingdom) and had resistances of 3–5 MΩ when filled with pipette solution. The pipette solution contained 120 mm KCl, 1 mm NaOH, 1 mm MgCl2, 1 mm CaCl2, 5 mm EGTA, 5 mm HEPES, and 0.3 mm K2ATP (pH adjusted to 7.3 with KOH; final [K+] approximately 140 mm). Whole cell currents were recorded at a holding potential of −20 mV and at 20°–24°C. Currents were evoked by repetitive 700-ms hyperpolarizing voltage ramps from −20 mV to −120 mV every 15 s and recorded using an EPC9 patch clamp amplifier (HEKA Elektronik, Lambrecht, Germany). Recordings were digitized at 0.5 kHz and analyzed using Pulse/Pulsefit software (HEKA) running on a personal computer. To confirm that all effects on the holding current at −20 mV were indeed caused by modulation of K+currents, reversal potentials were determined for each experimental condition and compared (table 1). There was no statistically significant difference in the reversal potential between the groups.
Concentration–response relations for the volatile anesthetics were obtained by alternating the control solution with a test concentration of anesthetic. The extent of inhibition by the anesthetic was then expressed as a fraction of the mean of the value obtained in the control solution before and after anesthetic application. Concentration–response curves were fitted to the Hill equation (equation 2):
where I is the holding current at −20 mV in the presence of the drug, Icis the current in the absence of the drug, [Vol] is the volatile anesthetic concentration, Kiis the anesthetic concentration at which inhibition is half maximal, and h is the slope factor (Hill coefficient).
Statistical analysis was performed using GraphPad Prism (GraphPad Software Inc., San Diego, CA). All data were expressed as mean ± SEM. To test for differences between groups, two-tailed unpaired t test or one-way analysis of variance followed by the Tukey multiple comparison test were used as appropriate. A value of P < 0.05 was considered significant.
Xenon but Not Sevoflurane Preconditioning Requires Functional Plasmalemmal KATPChannels
The current study was designed to analyze the role of KATPchannels in preconditioning induced by xenon and sevoflurane using OGD in neuronal–glial cocultures as an in vitro model of ischemic brain injury (fig. 1). In this model, 70–80 min of OGD was sufficient to maximally damage neurons, with glial cells being left largely unharmed. The extent of the injury was found to remain unchanged from 6 to 24 h after OGD, with no further evidence for either a delayed second burst of damage or repair mechanisms taking place.32
Exposure to the preconditioning anesthetics xenon or sevoflurane or to the potassium channel opener diazoxide 24 h before the OGD insult effectively prevented neuronal cell loss (survival: 80–100%; figs. 1B–D). The addition of the KATPchannel inhibitor tolbutamide to the xenon group during preconditioning completely abolished the protective effect of xenon (fig. 1B). Xenon's protective effect was also slightly reduced by the addition of the mito K-ATP channel inhibitor 5-hydroxydecanoate (5-HD). Although statistically significant, the reversal was not complete, because cell viability remained high in cultures treated concomitantly with xenon and 5-HD (fig. 1B). In contrast, the preconditioning effect of sevoflurane could not be reversed with either the KATPchannel inhibitor tolbutamide or the mito K-ATP channel inhibitor 5-HD (fig. 1C). Finally, diazoxide preconditioning was completely abolished by 5-HD and to a slightly lesser extent by tolbutamide (fig. 1D).
Diazoxide, at a concentration of 10 μm, is widely seen as specific for mito K-ATP channels. However, this is only true for cardiac tissue where KATPchannels have a SUR2A subunit. The SUR1 subunit of neuronal KATPchannels also responds to diazoxide. Therefore, it is not surprising that the preconditioning effect of diazoxide was sensitive to the KATPchannel blocker tolbutamide as well as the mito K-ATP channel antagonist 5-HD, suggesting a role for both channels.
These results indicated that opening of plasmalemmal KATPchannels, but not mito K-ATP channels, is essential for neuronal preconditioning by xenon, and demonstrated that sevoflurane preconditioning does not involve the opening of either plasmalemmal KATPchannels or mito K-ATP channels.
Evaluation of the Effects of Volatile Anesthetics on KATPCurrents
Plasmalemmal KATPchannels exist in a wide variety of organs, but their subunit composition differs between tissues. For example, neurons and pancreatic β cells carry channels mostly composed of Kir6.2 and SUR1 subunits, whereas myocardial and skeletal muscle have channels made up of Kir6.2 and SUR2A.33–35Consequently, it is not easily possible to extrapolate functional data and physiologic pathways related to KATPchannel activation from one organ to the other (e.g. heart to brain). Here, we used Kir6.2 and SUR1 as the components for KATPchannels because these are the subunits of KATPchannels in most neurons. HEK293 cells were transiently transfected with Kir6.2 and SUR1 complementary DNA. In contrast to untransfected HEK293 cells, these cells exhibited a large standing outward current at −20 mV, had a resting potential more negative than −65 mV, and were sensitive to tolbutamide, consistent with the expression of KATPchannels (fig. 2). During the first 5 min of whole cell voltage clamp recordings, an increase of outward current was observed consistent with the washout of adenosine triphosphate from the cytosol and subsequent progressive opening of plasmalemmal KATPchannels. This was then followed by a stable holding current of 1.05 ± 0.12 nA (n = 30) in Kir6.2 and SUR1–transfected HEK293 cells (figs. 2A and B). This holding current was inhibited reversibly by the addition of the specific KATPchannel blocker tolbutamide (100 μm; n = 17; figs. 2A and C). The zero-current potential for Kir6.2 and SUR1–transfected HEK293 cells was −77 ± 2 mV (n = 30), consistent with the fact that most of the whole cell conductance was made up by KATPchannels. In contrast, untransfected HEK293 exhibited a zero-current potential of −40 ± 5 mV and a holding current of 22 ± 10 pA at −20 mV (n = 13). This current was not enhanced by the K+channel opener diazoxide (200 μm; n = 6), consistent with the absence of functional KATPchannels in untransfected HEK293 cells.
Addition of sevoflurane to the superfusate reduced the KATPcurrent reversibly in a concentration-dependent manner (figs. 2A and C). This lack of activation of KATPcurrent by sevoflurane at clinically relevant concentrations (0.3–2.5 mm = 0.8–7.5 MAC) was consistent with the lack of effect of KATPchannel inhibitors on the preconditioning effect of sevoflurane. Next, the effects of sevoflurane were compared with those of two other volatile anesthetics: halothane and isoflurane. At a concentration of 1 mm, halothane had the strongest inhibitory effect on whole cell KATPcurrents, followed by isoflurane, and the smallest effect by sevoflurane (figs. 3A and B). This difference in potency was also reflected in the concentration–response curves for the different drugs (fig. 3C). Halothane inhibited KATPcurrents with an IC50of 1.3 ± 0.4 mm, isoflurane had an IC50of 2.1 ± 0.6 mm, and the effect of sevoflurane was extrapolated to an IC50of approximately 50 mm.
Next, the effects of xenon were tested on KATPcurrents. Xenon was applied at two concentrations: 50% and 80%. An 80% xenon solution is equivalent to 1 MAC or 3.4 mm xenon. Consequently, 50% xenon equates to 0.6 MAC and 2.1 mm. HEK293 cells transfected with Kir6.2 and SUR1 showed an increase in outward current by 19 ± 7% when superfused with a 50% xenon solution (n = 5) and by 44 ± 7% (n = 5) when exposed to 80% xenon solution as compared with control solution (80% N2; fig. 4). The reversal potential of this current (fig. 4Cand table 1) indicated it being a K+current. Furthermore, the current was inhibited by 0.1 mm tolbutamide (figs. 4C and D), and no increase in outward current in response to 80% xenon was observed in untransfected HEK293 cells (n = 5). These results strongly suggest that the xenon-induced K+current was due to the opening of Kir6.2/SUR1 channels. This activation of plasmalemmal KATPchannels was consistent with the preconditioning effect seen in the neuronal–glial cocultures being KATPchannel dependent.
Lack of Modulation of KATPChannels via Mitochondrial KATPChannels or by Drugs that Act on These
We next performed a series of experiments to demonstrate that the activity of KATPchannels in HEK293 cells is not significantly modulated by mito K-ATP channels under our experimental conditions. First, whereas the KATPchannel antagonist tolbutamide decreased current amplitude dramatically, no significant reduction in whole cell current was observed using the mito K-ATP channel inhibitor 5-HD (fig. 5). Equivalent results were obtained when using KATPchannel openers (fig. 6). Diazoxide and pinacidil have both been reported to open mito K-ATP channels,36,37but in addition, diazoxide activates KATPchannels containing SUR1, and pinacidil activates KATPchannels containing SUR2.38Consequently, diazoxide is expected to be mito K-ATP channel specific in systems that do not contain SUR1 (e.g. , heart muscle), and pinacidil would be specific for mito K-ATP channels in tissues not containing SUR2 (e.g. , most neurons). In HEK293 cells expressing Kir6.2 and SUR1, pinacidil did not increase the whole cell current significantly (figs. 6B and C). We took this as an indication that opening of mito K-ATP channels does not modulate KATPcurrents in these cells. In contrast, diazoxide concentration-dependently increased the whole cell current (figs. 6A and C) in accord with its direct effect on KATPchannels containing SUR1. In fact, at a concentration of 10 μm, diazoxide was able to stimulate the KATPcurrent to a similar extend as 80% xenon (fig. 6C). Because both of these drugs effectively precondition at these concentrations, one might postulate that an increase in KATPcurrent by approximately 50% is sufficient to initiate preconditioning. However, because diazoxide is known as a potent activator of mito K-ATP channels, it was explored whether mito K-ATP channel activation and subsequent alterations in mitochondrial function might contribute significantly to the KATPcurrent seen with 10 μm diazoxide. To test this hypothesis, the KATPcurrent was enhanced by 10 μm diazoxide and then 5-HD was added. No significant reduction of the diazoxide-elicited current was observed under these conditions (fig. 6D). These results established that 10 μm diazoxide activates KATPchannels independently from its effects on mito K-ATP channels. Taken together, these results provide strong evidence that the effects of volatile anesthetics on KATPwhole cell currents observed in this study are not secondary to the interaction of these drugs with mito K-ATP channels.
Neuronal Preconditioning by Anesthetics
The current study demonstrated that the mechanisms by which neuronal preconditioning is achieved can vary between individual inhalational anesthetics. More precisely, we were able to identify for xenon a pathway which was dependent on opening of plasmalemmal KATPchannels. Conversely, sevoflurane preconditioning was plasmalemmal KATPchannel independent. Importantly, neither of these anesthetics showed a substantial involvement of mito K-ATP channels in its preconditioning action. This lack of effect cannot be due to pathologic changes in our preparation because the control preconditioning with diazoxide, which acts in neurons on both plasmalemmal KATPchannels and on mito K-ATP channels, was indeed impaired by both the KATPchannel antagonist tolbutamide and the mito K-ATP channel blocker 5-HD. Given the dependence of ischemic preconditioning on functional plasmalemmal KATPchannels, as demonstrated by the lack of this preconditioning in cardiac muscle of Kir6.2−/−mice,8it seems as if (1) xenon mimics ischemic preconditioning and (2) sevoflurane acts on a different target. Whether this target is downstream from the activation of KATPchannels or involves an entirely independent pathway for preconditioning is unclear. A similar observation has been made in cerebellar brain slices, where blocking KATPchannels had no effect on isoflurane preconditioning.39Similarly to these results, Marinovic et al. 40reported that cardiac cytoprotection did not involve sarcolemmal KATPchannel opening during the preconditioning phase with isoflurane.
Anesthetic Effects on Recombinant Neuronal Plasmalemmal KATPChannels
Contribution of Mitochondrial K-ATP Channels.
Activation of mito K-ATP channels would be expected to dissipate the mitochondrial membrane potential, thus causing a reduction in adenosine triphosphate production.37,41With plasmalemmal KATPchannels being archetypal adenosine triphosphate sensors,38it would be expected that this decrease in adenosine triphosphate production would lead to channel activation and an increase in outward current (e.g. , as seen with cyanide exposure). However, our observation that neither pinacidil nor 5-HD had any effect on the activity of plasmalemmal KATPchannels indicates that modulation of mito K-ATP cannot influence plasmalemmal KATPchannels in our system. Therefore, the observed effects of anesthetics on these channels cannot be explained by an indirect effect via mito K-ATP channels.
Direct Effects on Plasmalemmal KATPChannels.
Probably the most interesting finding of this study was that the noble gas xenon acts as a K-channel opener. In previous studies that were primarily aimed at identifying the target for xenon's anesthetic action, this noble gas has been identified as an antagonist for the glycine binding site on N -methyl-d-aspartate receptors,42and it has been shown that xenon activates selective two-pore-domain potassium channels31(for review, see Preckel et al. 43). Here, we have demonstrated that the tolbutamide-sensitive preconditioning with xenon is mirrored by the activation of plasmalemmal KATPchannels by xenon at 1 MAC. At this concentration, xenon activated KATPchannels as efficiently as the specific KATPchannel opener diazoxide at its preconditioning concentration of 10 μm. Our results can be seen as indication that an increase in KATPchannel activity by 50% is sufficient to trigger preconditioning responses. They also clearly demonstrate that the neuroprotective effect of xenon is achieved at anesthetic or even subanesthetic concentrations and thus can be accomplished with clinically safe doses.
In contrast to xenon, sevoflurane did not precondition in a KATPchannel–dependent manner, and sevoflurane also did not activate plasmalemmal KATPchannels. In fact, slight inhibition was observed. Similar results were also found for isoflurane and halothane. Both of these inhibited the plasmalemmal KATPchannel mildly at 1 MAC, but more substantially than sevoflurane at higher concentrations. Similarly, it has previously been shown that barbiturates inhibit neuronal KATPchannels at supraclinical concentrations.44
A recent study investigating the acute effects of 4% sevoflurane on the membrane potential of hippocampal CA1 pyramidal cells also did not see an activation of KATPchannels despite the fact that hypoxia elicited such a hyperpolarization, which was also enhanced after preexposure to sevoflurane.45These results probably reflect our finding that sevoflurane is able to precondition, but not in a KATPchannel–dependent manner. Inhibition by halogenated anesthetics might be a general feature of inwardly-rectifying K+channels, because several members of this ion channel family were inhibited to varying degrees by these agents.46In the case of the KATPchannel, the SUR subunit might have an additional modulatory influence on the anesthetic sensitivity, because Bienengraeber et al. 47reported that the SUR2A subunit of cardiac sarcolemmal KATPchannels conferred isoflurane activation of the K+current under acidic conditions.
Physiologic Significance of KATPChannel Inhibition
Here, we have shown that halogenated anesthetics inhibit plasmalemmal KATPchannels. This should have little effect because KATPchannels are closed under physiologic conditions in most tissues. They would only open under conditions of metabolic stress, such as ischemia. However, a notable exception is the pancreatic β cell, where KATPchannel opening controls the glucose-dependent insulin release.48Consequently, inappropriate KATPchannel inhibition could potentially lead to hyperinsulinemia and hypoglycemia. In addition, patients who take antianginal medication such as the K-channel opener nicorandil or antihypertensives such as cromakalim or pinacidil might lose some protection if exposed to drugs that inhibit KATPchannels.49,50
The halogenated volatiles tested here had inhibitory effects on KATPcurrents at 1 MAC (fig. 3), but currently there are not sufficient data to allow a critical evaluation of potential interactions between anesthetics and K-channel openers. Furthermore, because it is unknown whether these drugs interact with the potassium channel subunit or the sulfonylurea receptor (SUR1 in this case), it is not clear whether the cardiac or the smooth muscle plasmalemmal KATPchannel is affected at all.
Physiologic Consequence of KATPChannel Activation
Conversely, drugs that open KATPchannels can potentially interfere with the sulfonylurea-induced insulin secretion in diabetic patients. However, our finding that tolbutamide prevents the opening of KATPchannels by xenon argues that on the contrary diabetes treatment might interfere with the organ-protective effect afforded by xenon. This is reminiscent of the interference of sulfonylurea drugs with the antianginal drug nicorandil.49Although this is a valid concern for peripheral tissue, the fact that tolbutamide does not easily partition into the brain51,52makes xenon a viable choice even for diabetic patients.
Most KATPchannel openers do not cross the blood–brain barrier under physiologic conditions. Nevertheless, studies have reported neuroprotective effects of these drugs in vivo . However, rather than exerting their effects directly on the neuronal plasma membrane, the observed effect might be secondary to increased cerebral blood flow due to the vasodilatory effect of these drugs. They open KATPchannels in vascular smooth muscle cells.53Similarly, xenon has been shown to stimulate cerebral blood flow54–56and to dilate pial vessels.57This might indicate that xenon activates KATPchannels of the smooth muscle subtype Kir6.1/SUR2B and raises the question of whether xenon differs from classic KATPchannel openers by having no, or a reduced, tissue specificity and thus works via a novel mechanism.
In summary, we have established xenon as a novel plasmalemmal KATPchannel opener (that can readily cross the blood–brain barrier) on both a molecular and a functional basis. Furthermore, we have demonstrated two distinct preconditioning pathways, one that is KATPchannel dependent and one that is not. Further studies are likely to reveal subtle differences in the protection afforded by the KATPchannel–dependent pathway that probably matches the naturally occurring ischemic preconditioning most closely, and the protection via the KATPchannel–independent pathway. This might open new doors for the treatment of stroke patients. Finally, xenon, with its favorable safety profile, might be the drug of choice to preoptimize patients before surgery, especially for procedures that carry some risk of inducing ischemic stroke, such as heart surgery or carotid endarterectomy.
The authors thank Mahmuda Hossain, Ph.D. (Technician, Department of Anaesthetics, Pain Medicine and Intensive Care, Chelsea and Westminster Hospital, Imperial College London, London, United Kingdom), and Cleoper Paule, Ph.D. (Research Student, Department of Anaesthetics, Pain Medicine and Intensive Care, Chelsea and Westminster Hospital, Imperial College London), for their technical support.