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Am J Physiol Heart Circ Physiol 286: H1339-H1346, 2004. First published December 4, 2003; doi:10.1152/ajpheart.00227.2003
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ET-1 induces cortical spreading depression via activation of the ETA receptor/phospholipase C pathway in vivo

Jörg Kleeberg, Gabor C. Petzold, Sebastian Major, Ulrich Dirnagl, and Jens P. Dreier

Departments of Neurology and Experimental Neurology, Humboldt University, 10117 Berlin, Germany

Submitted 13 March 2003 ; accepted in final form 25 November 2003


   ABSTRACT
TOP
 ABSTRACT
MATERIALS AND METHODS
 RESULTS
 DISCUSSION
 REFERENCES
 
Recently, it has been shown that brain topical superfusion of endothelin (ET)-1 at concentrations around 100 nM induces repetitive cortical spreading depressions (CSDs) in vivo. It has remained unclear whether this effect of ET-1 is related to a primary neuronal/astroglial effect, such as an increase in neuronal excitability or induction of interastroglial calcium waves, or a penumbra-like condition after vasoconstriction. In vitro, ET-1 regulates interastroglial communication via combined activation of ETA and ETB receptors, whereas it induces vasoconstriction via single activation of ETA receptors. We have determined the ET receptor profile and intracellular signaling pathway of ET-1-induced CSDs in vivo. In contrast to the ETB receptor antagonist BQ-788 and concentration dependently, the ETA receptor antagonist BQ-123 completely blocked the occurrence of ET-1-induced CSDs. The ETB receptor antagonist did not increase the efficacy of the ETA receptor antagonist. Direct stimulation of ETB receptors with the selective ETB agonist BQ-3020 did not trigger CSDs. The phospholipase C (PLC) antagonist U-73122 inhibited CSD occurrence in contrast to the protein kinase C inhibitor Gö-6983. Our findings indicate that ET-1 induces CSDs through ETA receptor and PLC activation. We conclude that the induction of interastroglial calcium waves is unlikely the primary cause of ET-1-induced CSDs. On the basis of the receptor profile, likely primary targets of ET-1 mediating CSD are either neurons or vascular smooth muscle cells.

endothelin-1; endothelin receptor antagonists; interastroglial calcium waves; gap junction communication; protein kinase C inhibition; arachidonic acid; cortical spreading depression

ENDOTHELIN (ET)-1 was initially believed to influence brain functions only indirectly through regulation of cerebral perfusion due to its vasoconstrictor activity. However, over the past few years, evidence has accumulated that ET-1 may fulfill a wider range of physiological actions within the central nervous system (CNS), which has also led to its recognition as a neuropeptide (for reviews, see Refs. 33 and 36). Beside neurons, astrocytes represent a major ET target. Several studies have shown that ET-1 affects numerous cell functions of cultured astrocytes such as control of ion channel activity (5), glutamate efflux (52) and uptake (41), glucose utilization (58), permeability of gap junction communications (3, 16), and calcium signaling (3, 64). In turn, astrocytes are a major source of ET-1 (12, 13) and seem to play an important role in the regulation of ET-1 levels within the CNS (14, 24, 25).

In contrast to the cerebrovascular system, in which ETA receptors are the major receptor subtype, astrocytes predominantly express the ETB receptor subtype (26, 38). However, at least in cultured astrocytes, there has also been evidence of ETA receptor mRNA expression (13) and an ETA/ETB hybrid receptor has been postulated (31). This unusual receptor pattern may be involved in certain actions of ET-1, such as increased glutamate efflux, evocation of calcium signaling, and controlling gap junction communication in cultured astrocytes (3, 52).

An interesting feature of astrocytes is their long-range signaling between themselves and neurons through intercellular gap junction-mediated calcium waves (18, 55). Such calcium waves can lead to depolarization of surrounding neurons and have been suggested to play a role in the initiation and propagation of cortical spreading depressions (CSDs) in in vitro models (Ref. 45; for a review, see Ref. 42). ET-1 is known to evoke such intercellular calcium waves in cultured astrocytes (3, 63) and regulates their expansion by gap junction channel closure (3, 16). Interestingly, these effects of ET-1 on astrocytes are only inhibited significantly if both ETA and ETB receptors are simultaneously blocked (3). This is in contrast to several ET-1 effects on the vasculature or neurons that are inhibited by the application of either ETA or ETB receptor antagonists (48, 59, 66, 67). In a complex system such as the brain in vivo, it may be difficult to decide which cellular targets/functions mediate the complex effect of ET-1 on the neuronal/astroglial network. Studying the receptor profile/intracellular signaling cascade using receptor agonists and antagonists may help to limit the number of candidate cell types and functions for a given network effect. Here, we applied such an approach to analyze the recently discovered potent and reliable generation of CSDs by ET-1 in vivo (8).


   MATERIALS AND METHODS
TOP
 ABSTRACT
 MATERIALS AND METHODS
RESULTS
 DISCUSSION
 REFERENCES
 
Animals

All animal experiments were approved by the Landesamt für Arbeitsschutz, Gesundheitsschutz, und Technische Sicherheit Berlin (G 0346/98). Male Wistar rats (n = 101, 280–380 g) were anesthetized with 100 mg/kg thiopental sodium intraperitoneally (Trapanal, BYK Pharmaceuticals; Konstanz, Germany), tracheotomized, and artificially ventilated (Effenberger Rodent Respirator, Effenberger; Pfaffing/Attel, Germany). The left femoral artery and vein were cannulated, and a saline solution (1 ml/h) was continuously infused. Body temperature was maintained at 38.0 ± 0.5°C using a heating pad. Systemic arterial pressure (RFT Biomonitor; Zwönitz, Germany) and end-expiratory PCO2 (Heyer CO2 Monitor EGM I; Bad Ems, Germany) were monitored. Arterial PO2, arterial PCO2, and pH were serially measured using a Compact 1 Blood Gas Analyzer (AVL Medizintechnik; Bad Homburg, Germany). Because the rats were not paralyzed, the adequacy of the level of anesthesia was assessed by testing motor responses to tail pinch. In addition, changes of blood pressure in response to tail pinch were used to control anesthesia. Further thiopental doses (25 mg/kg ip) were applied when necessary.

A craniotomy was performed over the parietal cortex using a saline-cooled drill. A closed cranial window was implanted as previously described (9). The dura mater was removed. The craniotomy site was covered with a piece of glass cut from a coverslip. An inflow and outflow tube allowed us to superfuse the brain cortex continuously with artificial cerebrospinal fluid (aCSF) at the closed window (Fig. 1). The composition of the aCSF was (in mM) 152 Na+, 3 K+, 1.5 Ca2+, 1.2 Mg2+, 24.5 , 135 Cl–, 3.7 glucose, and 6.7 urea. The aCSF was equilibrated with a gas mixture containing 6.6% O2-5.9% CO2-87.5% N2. PO2 between 90 and 130 mmHg, PCO2 between 35 and 45 mmHg, and pH between 7.35 and 7.45 were accepted as physiological. Regional cerebral blood flow (CBF) was continuously monitored with a laser-Doppler flow probe (Perimed; Järfälla, Sweden). The steady [direct current (DC)] potential was measured with an Ag-AgCl electrode in the subarachnoid space. Electrodes were connected to a differential amplifier (Jens Meyer; Munich, Germany). The subarachnoid DC potential changes associated with CSDs are smaller but correlate well with intracortical DC potential changes as measured with microelectrodes in the cranial window area (8). In contrast to an open cranial window, a closed cranial window does not allow use of microelectrodes but has other advantages such as control of intracranial pressure and more stable PCO2 levels. CBF and DC potential were continuously recorded using a personal computer and chart recorder (DASH IV, Astro-Med; West Warwick, RI).



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  		Fig. 1. Experimental setup. The closed window was covered by a piece of glass cut from a coverslip. An inflow (aCSFin) and outflow tube (aCSFout) allowed the superfusion of the cortex with artificial cerebrospinal fluid (aCSF) containing the drugs used. Cerebral blood flow (CBF) was measured by one laser-Doppler flow probe (LDF) at the window. The direct current (DC) shift was recorded using an Ag-AgCl electrode.

 

Experimental Protocols

General procedures for groups 1 and 2. The drugs were first administered alone and then coapplied with increasing concentrations of ET-1 from 10 nM to 1 µM in the aCSF. Equilibration time was 1 h for each application. The number of animals is given in parentheses.

ET receptor antagonists (group 1). The drugs tested were the ETA receptor antagonist BQ-123 topically applied at 500 nM (n = 7), 1 µM (n = 6), 5 µM (n = 6), and 50 µM (n = 6); the ETB receptor antagonist BQ-788 at 500 nM (n = 7), 5 µM (n = 6), and 50 µM (n = 10); BQ-123 at 500 nM together with BQ-788 at 5 µM (n = 6); and the ETB receptor agonist BQ-3020 at 1 µM (n = 6). The results of these 60 experiments were compared with 12 control experiments in which ET-1 was continuously superfused in increasing concentrations from 10 nM to 1 µM without receptor antagonist or agonist.

Phospholipase C inhibitor U-73122 and PKC inhibitor Gö-6983 (group 2). To study the intracellular pathways after ET receptor activation, U-73122 in 1% DMSO was coapplied with ET-1 (10 nM–1 µM) in 10 animals and Gö-6983 in 1% DMSO in another 6 animals. These results were compared with a vehicle control in which 1% DMSO was coapplied with increasing concentrations of ET-1 from 10 nM to 1 µM (n = 7).

Arachidonic acid (group 3). aCSF containing arachidonic acid at a concentration of 100 µM and 1 mM was brain topically applied in six animals. The application time for each concentration was 1 h.

Chemicals and Drugs

Gö-6983 was obtained from Calbiochem (Beeston/Nottingham, UK), BQ-3020 was from Alexis (Lausen, Switzerland), and all other chemicals were purchased from Sigma (Deisenhofen, Germany).

Statistical Methods

Data were analyzed by comparing relative changes of CBF and absolute changes of the DC potential. CBF changes were calculated in relation to baseline at the onset of the experiment (equal to 100%). A zero level was established at the end of the experiments after global cerebral ischemia. All data are given as means ± SD. Statistical comparisons were performed using Fisher's exact test, ANOVA with repeated measures with Scheffé's post hoc test or one-way ANOVA with Bonferroni's post hoc test. A value of P < 0.05 was considered as statistically significant.


   RESULTS
TOP
 ABSTRACT
 MATERIALS AND METHODS
 RESULTS
DISCUSSION
 REFERENCES
 
Systemic Variables

Systemic variables remained within physiological limits throughout the experiments. The physiological variables during the experiments are shown in Table 1.


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  		Table 1. Physiological variables after the experiments

 

Group 1: Receptor Profile of ET-1-Induced CSDs

ET-1 induced CSDs in a concentration-dependent manner in the absence of any ET receptor agonist or antagonist. In 2 of 12 animals, ET-1 induced CSDs at 10 nM. Ten of the animals generated CSDs at 100 nM. All animals developed CSDs when ET-1 was increased to 1 µM (shown as the control in Fig. 3, A, B, and D). CBF increased to 186 ± 65% during the first CSD. The hyperemia lasted for 86 ± 20 s. CSD was associated with a negative subarachnoid DC shift of –3.8 ± 1.8 mV lasting for 79 ± 22 s. The CSD frequency was 5 ± 3 per hour (range: 1–10). An example of original traces of the changes of CBF and DC potential during CSD in response to ET-1 is shown in Fig. 2. Similar experiments were carried out and analyzed in detail concerning CBF, intracortical and subarachnoid DC potentials, and extracellular K+ concentration ([K+]o) changes as well as propagation in a previous study (8).



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  		Fig. 3. A: to determine the ET receptor involved in the generation of CSD, the ETA receptor antagonist BQ-123 was coapplied with increasing concentrations of ET-1 from 10 nM to 1 µM in 25 animals. It is shown that BQ-123 dose dependently abolished the generation of CSDs by ET-1. Complete blockade was achieved at a concentration of 5 µM. The statistical comparison was performed using a Fisher's exact test (drug compared with control under the same ET-1 concentration, *P < 0.05). In addition, BQ-123 abolished the ET-1-induced CBF decrease, which was statistically tested for each concentration of BQ-123 using ANOVA with repeated measures with the Scheffé's post hoc test (*P < 0.05 and **P < 0.01). At a BQ-123 concentration of 50 µM, ET-1 induced vasodilation. This was probably related to the activation of vasodilative ETB receptors while the vasoconstrictive ETA receptors were blocked. The CBF values are average values over the last 5 min before we washed in the next drug cocktail. We have previously shown that the baseline drift over long recording periods is not significant in our model (10). B: similarly to BQ-123, the ETB receptor antagonist BQ-788 was coapplied with increasing concentrations of ET-1. At a concentration of 50 µM, a partial blockade of CSD generation by ET-1 was observed. Interestingly, at this concentration, BQ-788 inhibited rather than augmented the ET-1-induced CBF decrease. Therefore, BQ-788 at 50 µM probably interfered with ETA receptors. C: the combination of BQ-123 at 500 nM together with BQ-788 at 5 µM was not more effective than either antagonist alone. D: direct stimulation of the ETB receptor with the selective agonist BQ-3020 at 1 µM did not trigger CSDs. Also, coapplication of BQ-3020 and ET-1 did not significantly change the percentage of animals exhibiting CSD despite increased CBF levels.

 


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  		Fig. 2. Example of original traces of the changes of CBF and DC potential during a cluster of cortical spreading depressions (CSDs) in response to endothelin (ET)-1 at a concentration of 100 nM. As can be seen in the top trace, CBF declines shortly before the first CSD starts. CBF then increases for ~1 min (hyperemia phase), followed by a decrease below the baseline (oligemia phase). A few minutes later, a second and third CSD occur. The bottom trace shows subarachnoid DC shifts typical of CSDs occurring simultaneously with the flow changes.

 

To determine the ET receptor subtype involved in the generation of CSD, BQ-123, BQ-788, or BQ-3020 were brain topically coapplied with increasing concentrations of ET-1 (10 nM–1 µM). Superfusion of BQ-123 dose dependently inhibited the generation of CSDs by ET-1 (Fig. 3A). CBF increased to 159 ± 57% and DC shifted to –3.3 ± 2.8 mV during the first CSD when ET-1 and BQ-123 (500 nM) were coapplied. CSD frequency was 6 ± 4 per hour (range: 1–12). At BQ-123 (1 µM), only two of six animals generated one to five CSDs in response to ET-1. CBF increased to 173 ± 57% and DC fell to –2.9 ± 0.9 mV in response to the first CSD. Complete blockade was observed when BQ-123 was applied at a concentration of 5 µM. In addition, the ETA receptor antagonist BQ-123 dose dependently abolished the CBF decrease induced by increasing concentrations of ET-1 (ANOVA with repeated measures with the Scheffé's post hoc test; Fig. 3A, n = 25). BQ-123, coapplied at a concentration of 50 µM, rendered ET-1 a vasodilator. This was probably related to activation of vasodilative ETB receptors when the ETA receptors were blocked. Therefore, 50 µM probably represented a saturating concentration (27).

Superfusion of the ETB receptor antagonist BQ-788 at a concentration of 500 nM and 5 µM did not inhibit the generation or changed the frequency of CSDs in response to increasing concentrations of ET-1. The hyperemia was 193 ± 67% and 216 ± 71%, respectively, during the first CSD. The negative DC shift was –2.7 ± 1.3 and –2.3 ± 1.6 mV, respectively. An inhibiting effect by BQ-788 was only achieved at a concentration of 50 µM (P < 0.01, Fisher's exact test; Fig. 3B, n = 23). However, at this concentration, BQ-788 is no longer selective for ETB receptors but also inhibits ETA receptors (29). The hyperemia was 204 ± 66%, and the negative DC shift was –2.5 ± 2.8 mV. The CSD frequency was 4 ± 3 per hour (range: 2–8). An interaction of BQ-788 with the ETA receptor may also explain why, at a concentration of 50 µM, BQ-788 did not augment but seemed to attenuate the ET-1-induced CBF decrease (Fig. 3B).

To study whether a combined action of ET receptors was significantly more effective than either of the ET receptors alone, BQ-123 and BQ-788 were also simultaneously applied at 500 nM and 5 µM, respectively (n = 6). This yielded a similar effect as a single application of BQ-123 at 500 nM (Fig. 3C). Therefore, a pronounced combined action of ETA and ETB receptors was excluded.

Superfusion of the ETB receptor agonist BQ-3020 did not induce CSDs at a concentration of 1 µM (Fig. 3D, n = 6). When BQ-3020 was coapplied with ET-1, the percentage of animals exhibiting CSDs did not change significantly (Fig. 3D, n = 6). CBF increased to 263 ± 59% during the first CSD. The associated negative DC shift was –4.5 ± 1.4 mV. The CSD frequency was 5 ± 3 per hour (range: 1–6). Interestingly, CSDs were induced by ET-1 in the presence of BQ-3020 despite increased average CBF levels compared with the controls (P < 0.05 and 0.01, respectively, two sample t-tests; Fig. 3D).

There was no statistically significant difference in frequency, hyperemic CBF level, or negative DC shift between ET-1-induced CSD in the presence or absence of BQ-123, BQ-788, and BQ-3020, respectively (one-way ANOVA with Bonferroni's post hoc test).

Group 2: Intracellular Pathways Possibly Involved in ET-1-Induced CSDs

The signal transduction pathway initiated by activated ET receptors appears to involve stimulation of phospholipase C (PLC). PLC leads to the formation of inositol (1,4,5)-trisphosphate [Ins(1,4,5)P3] and diacylglycerol (DAG), which are the starting points for several intracellular signal cascades. One Ins(1,4,5)P3-mediated signal cascade involves an increase of the intracellular Ca2+ concentration, which in turn mediates, e.g., constriction of vascular smooth muscle (VSM) (19) or intercellular Ca2+ waves within the astroglial syncytium induced by ET-1 (63, 64). To determine the role of PLC in the process of CSD generation by ET-1, we topically coapplied the PLC inhibitor U-73122 at a concentration of 50 µM together with increasing concentrations of ET-1. U-73122 significantly reduced the percentage of animals exhibiting ET-1-induced CSDs (n = 10) compared with vehicle-treated animals (n = 7) (P < 0.01, Fisher's exact test; Fig. 4).



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  		Fig. 4. The signal transduction pathway initiated by ET receptors has been shown to involve phospholipase C (PLC) in both vascular smooth muscle and astrocytes. It is shown that the PLC inhibitor U-73122 significantly inhibited CSD generation by ET-1 compared with the vehicle control (*P < 0.05). In contrast, the PKC inhibitor Gö-6983 had no significant effect.

 

DAG and intracellular calcium stimulate PKC. Therefore, we coadministered the PKC inhibitor Gö-6983 at a concentration of 10 µM together with increasing concentrations of ET-1. Gö-6983 did not affect the generation of CSDs by ET-1 (n = 6; Fig. 4).

Group 3: Does ET-1 Induce CSDs Via Release of Arachidonic Acid?

ET-1 is also known to stimulate the arachidonic acid metabolism via activation of phospholipases. For example, it has been proposed that interastroglial metabolic trafficking is inhibited via this pathway (58). Failure of energy metabolism is known to promote CSDs. Therefore, it was tested whether topical superfusion of aCSF containing arachidonic acid at a concentration of 100 µM and 1 mM induced CSD. No such effect was observed (n = 6). Arachidonic acid increased CBF to 127 ± 15% and 148 ± 30%, respectively.


   DISCUSSION
TOP
 ABSTRACT
 MATERIALS AND METHODS
 RESULTS
 DISCUSSION
REFERENCES
 
General

Recently, it has been shown that the endothelial factor ET-1 is the most potent inductor of CSDs in vivo currently known (8). This finding may have particular relevance for the pathophysiological understanding of migraine, because several clinical lines of evidence suggest that, in a fraction of patients, endothelial irritation may somehow lead to migrainous aura and ET-1 may be involved in migraine (8, 60). The mechanism by which ET-1 induces CSDs has remained enigmatic. It is not even clear which cellular target of ET-1 mediates that action. Possible cellular targets are astroglial cells, neurons, or VSM. Altered function of astrocytes could lead to CSDs via, e.g., interastroglial calcium waves, altered function of neurons via a change in excitability or energy metabolism, or of VSM via a penumbra-like condition (8). That ET-1 did not induce CSD in neocortical brain slices seems to contradict the hypothesis that astrocytes or neurons are the primary targets of ET-1. That CBF only mildly decreased before ET-1-induced CSD seems to contradict VSM as the primary target (8).

Interastroglial Communication and CSDs

Interastroglial calcium waves have been proposed as the cellular correlate of CSDs because both phenomena can occur simultaneously and propagate at a similar rate (28, 35, 45, 46). Therefore, it is an attractive hypothesis that induction of interastroglial calcium waves by ET-1 may underlie ET-1-induced CSDs. The receptor profile of ET-1 controlling interastroglial calcium communication is known (3): both ETA and ETB receptor need to be blocked to inhibit that action of ET-1. The intracellular signal transduction pathway includes PLC activation leading to formation of Ins(1,4,5)P3. This, in turn, releases calcium from Ins(1,4,5)P3-sensitive internal stores (18, 63, 64). Also, the kinetics of the regulatory action of ET-1 on astroglial communication is known: short-term application of ET-1 triggers an interastroglial calcium wave in vitro, whereas prolonged exposure with ET-1 inhibits gap junction communication and propagation of calcium waves (3, 18, 63).

We found that the PLC inhibitor U-73122 antagonized the initiation of CSDs by ET-1. However, PLC is also involved in several ET-1-related effects other than the induction of calcium waves. For example, inhibition of PLC by neomycin partially blocked ET-1-induced vasoconstriction in rat cerebral arteries in vitro (19). In addition, ET-1 induced a transient calcium release via Ins(1,4,5)P3 from the sarcoplasmic reticulum and a sustained release related to receptor-operated calcium-permeable channels of the plasma membrane in rabbit cortical arterioles (22). Similar transient intracellular calcium increases, dependent on the endoplasmic reticulum, and sustained increases, dependent on extracellular calcium, were also induced by ET-1 in neurons (34, 67).

Two of our findings contradict the notion that the initiation of interastroglial calcium waves is responsible for ET-1-induced CSDs; one argument is based on the kinetics of both processes. If ET-1 induced CSDs via initiation of an interastroglial calcium wave, we would expect that only one CSD would occurred. After the first, further CSDs would not arise because gap junctions would be blocked. However, we observed repetitive CSDs over a period of at least 2 h in the presence of ET-1. The second argument is related to the receptor profile: combined application of both ET receptor antagonists was not necessary to inhibit CSD generation in our study. Instead, we found that ETA receptor activation mediated CSD generation. The ETB receptor antagonist only inhibited the occurrence of CSDs at an unselectively high concentration (29). We confirmed that the ETB receptor was not involved because the ETB receptor agonist BQ-3020 did not induce CSDs. Whereas the ETA receptor mediating CSD makes a primary astroglial target of ET-1 unlikely, it is known that ET-1 can release intracellular calcium via that receptor subtype in both VSM and certain neurons, suggesting a link between ETA receptor activation and PLC in VSM and neurons (22, 67).

PLC activation may not necessarily lead to CSDs via Ins(1,4,5)P3 production. Another product of PLC activation is DAG. DAG and intracellular calcium stimulate PKC. A role for PKC has been suggested, e.g., in ET-1-induced vascular contraction (19, 21). However, the PKC inhibitor Gö-6983 was not able to inhibit the generation of CSD by ET-1. This finding suggests that PKC activation did not represent a critical step in the cascade leading to CSDs.

Via activation of phospholipases, ET-1 is also known to stimulate arachidonic acid metabolism. Interestingly, both arachidonic acid and ET-1 uncouple gap junctions (16, 17, 58). In vitro, uncoupling of gap junctions led to inhibition of CSD when long-chain alkyl alcohols were applied (35, 46), whereas another potent uncoupling agent, carbenoxolone, had no effect on CSDs (65). The discovery that a potent gap junction blocker such as ET-1 is a highly potent inductor of CSDs is indeed surprising. A possible explanation could be related to a disturbance of interastroglial metabolic trafficking via gap junction blockade. Thus, with the use of a scraped monolayer of cultured astrocytes, it was shown that arachidonic acid at 50 µM blocked the diffusion of radioactively labeled glucose, glucose-6-phosphate, and lactate through gap junctions similarly to ET-1 at 100 nM, octanol at 600 µM, or {alpha}-glycyrrhetinic acid at 200 µM (17, 58). In vivo, but not in brain slices, inhibited metabolic trafficking could interfere with neuronal nutrition because astrocytes may constitute a physical barrier in the supply of metabolic substrates from blood to neurons (49). A decreased supply of energy substrates is known to promote CSDs. In addition, CSD-like depolarizations under the condition of energy compromise are less sensitive to gap junction blockade with long-chain alkyl alcohols (1). Earlier, it was already suggested that arachidonic acid could be involved in the mechanism underlying CSDs (39). However, we found that arachidonic acid, even at high concentrations, did not induce CSDs in vivo, in contrast to ET-1. This finding did not support the hypothesis that inhibited metabolic trafficking was critically involved in ET-1-induced CSDs.

In addition to these findings specifically related to ET-1-induced CSD, there are several more general arguments against interastroglial communication being crucial for the generation or propagation of CSDs (for a review, see Ref. 56). Thus Basarsky et al. (2) showed that CSDs in calcium-free medium also occurred in the absence of intercellular calcium waves. In addition, metabolic poisons for astroglial cells, fluoroacetate and fluorocitrate, did not prevent CSDs but rather facilitated their onset (37).

The increase of CBF by arachidonic acid may be related to the formation of epoxyeicosatrienoic acids by astrocytes (23) or direct activation of tandem pore domain potassium channels in VSM (6).

CSD-Like Depolarizations and a Penumbra-Like Condition

Because ET-1 is a potent vasoconstrictor, it appears possible that CSD-like depolarizations are triggered through an ischemic penumbra-like condition. This hypothesis has been extensively discussed in an earlier study (8). In brief, arguments in support were 1) that ET-1 did not induce CSD in brain slices; 2) that small increases in [K+]o preceded ET-1-induced CSDs similar to those observed before CSD-like depolarizations in an ischemic penumbra (43, 47); and 3) that a nitric oxide (NO) donor shifted the threshold concentration of ET-1 initiating CSDs to a higher level, whereas neither initiation nor propagation of CSDs triggered by needle stab was affected by a NO donor (32). The main argument against the vascular theory was that ET-1 decreased CBF only slightly before it induced CSDs (8). In the present study, we showed that ET-1 even induced CSDs even though CBF was above baseline when we coapplied the ETB receptor agonist BQ-3020. An earlier report, using topical application of ET-1 to the brain surface, consistently showed that the threshold concentration of ET-1 producing ischemia in a large tissue volume is above the range that, in our model, led to CSDs (15). However, the laser-Doppler flow probe measures CBF in a rather large volume of ~1 mm3. It is possible that the flow distribution in the tissue is heterogeneous and a very small ischemic region, e.g., at the cortical surface, remains undetected. In our study, the receptor profile of ET-1-induced CSDs is consistent with that of the vasoconstrictor action of ET-1. Therefore, in contrast to the astroglial theory, it remains a possibility that the vascular action of ET-1 is involved in the generation of CSDs. This issue has to be addressed in a future study. Another vascular hypothesis to investigate is related to the question of whether disruption of the blood-brain barrier (BBB) by ET-1 may promote the induction of CSD. Consistently, similar to vasoconstriction, BBB opening by ET-1 is mediated via ETA receptors (44, 57). Furthermore, it has recently been shown that BBB disruption causes changes in neuronal excitability (53). It deserves further study as to whether these changes are relevant for the initiation of CSDs by ET-1. Alternatively to the vascular hypothesis, the receptor profile of ET-1-induced CSDs leaves the possibility that ET-1 triggers CSDs via a direct action on neurons, e.g., related to augmentation of glutamatergic neurotransmission (54).

In general, in this discussion, when comparing the CSD threshold in response to ET-1 with other ET-1-related effects, it is necessary to consider the influence of different anesthetics in vivo. For example, thiopental is known to reduce both neuronal metabolism and baseline CBF (11). These actions possibly lower the CSD threshold. In contrast, other anesthetics may increase the CSD threshold either by inhibiting CSDs directly or by antagonizing ET-1. Halothane is such a candidate. It is known to inhibit ET-1 effects directly such as vasoconstriction in rat aortic rings or astroglial Ca2+ increases in cell culture (4, 63). In addition, it seems to directly interfere with CSD initiation (51). These issues have to be addressed in a future study.

Relation Between ET-1- and K+-Induced CSDs

Leão (40) described CSDs in 1944 as a wave of depression of "spontaneous" electrocorticographic activity that propagated in the rabbit cortex. Several theories on the mechanism of CSD initiation and propagation later evolved [reviewed by Somjen (56)]. Grafstein (20) and van Harreveld and Fifkova (62) coined the two most influential theories: the "potassium" and "glutamate" theories. Grafstein proposed that K+ released from neurons during intensive firing accumulates in the extracellular space. This increase in interstitial K+ would further depolarize the firing neurons leading to a vicious circle resulting in the depression of neuronal excitability. Simultaneously, the released K+ would diffuse to neighboring neurons, there giving rise to the cycle of depolarization followed by neuronal inactivation. Although some aspects of this theory such as a critical role for action potential firing were not confirmed in later studies, the core of the theory has survived. Particular evidence exists that an increase in interstitial K+ is important in the ignition and evolution of CSD rather than its propagation (56). The van Harreveld glutamate theory was based on the findings that this amino acid can induce CSDs, it is released during CSDs and the Na+ channel blocker tetrodotoxin suppresses action potential firing but neither inhibits CSD nor glutamate release during CSDs nor glutamate's excitatory action. The glutamate theory was later supported by the observation that N-methyl-D-aspartate (NMDA) receptor antagonists inhibit CSD propagation in normal tissue (56).

The very initial cascade of ET-1- and K+-induced CSDs must be different because ET-1 does not induce CSDs in brain slices, in contrast to K+. However, there are also similarities between the two inductors of CSDs. Thus the repolarization of K+-induced CSDs is prolonged at the initiation site both in vivo and in vitro similar to the repolarization of ET-1-induced CSDs in vivo (8). Second, K+-induced CSD is preceded by an artificial increase in baseline [K+]o at the initiation site; ET-1-induced CSD is also preceded by a gradual rise in baseline [K+]o, although this occurs spontaneously, similarly as in hypoxic CSD in brain slices (43) or periinfarct depolarizations in vivo (47). Hypothetically, the combination of a rise in baseline [K+]o preceding CSD and a prolonged repolarization phase represent two key features characterizing the initiation site of CSD in general, independent of the CSD-inducing agent. Consistent with a distinct pathogenetic situation between initiation and propagation sites, NMDA receptor antagonists less potently inhibit initiation of CSD than its propagation in surrounding normal tissue (56). The gradual rise in baseline [K+]o at the initiation site may be related to opening of K+ channels (43) and downregulation of the Na+-K+-ATPase activity (10), whereas the latter may also be responsible for the delay in repolarization.

ET-1 causes a small rise in baseline [K+]o in vivo but not in brain slices before CSD. This is again consistent with a link between the gradual rise in baseline [K+]o and the initiation of CSD as discussed above. On the basis of this notion, we speculate that the key for understanding the mechanism underlying ET-1-induced CSD is hidden in the process by which ET-1 causes the gradual rise in baseline [K+]o. Consistent with the above hypothesis regarding Na+-K+-ATPase, we have recently shown that ET-1 downregulates Na+-K+-ATPase activity in vivo even before CSD starts (50). This mainly occurs on account of the {alpha}2/{alpha}3 activity. The reasons are unknown for the decrease in Na+-K+-ATPase activity. Possibly, perturbations in membrane integrity and/or association of the {alpha}-isoforms of this enzyme are responsible (30).

In conclusion, based on the identified ET receptor profile in this study, we conclude that either VSM cells or neurons, but not astroglial cells, constitute the likely primary targets of ET-1 to induce CSD. Following this conclusion, ET-1 would depolarize neurons either via direct action or as a consequence of decreased energy supply due to contracted VSM. The special features of ET-1 may be particularly interesting with respect to clinical conditions that often present with both migraine aura and stroke, such as cerebral autosomal dominant arteriopathy with subcortical infarcts and leukoencephalopathy (7) or hereditary infantile hemiparesis, retinal arteriolar tortuosity, and leukoencephalopathy (61).


   ACKNOWLEDGMENTS
 
GRANTS

This study was supported by German Research Foundation Grant DFG-SFB 507 A1 (to J. P. Dreier and U. Dirnagl). The support of the Hermann and Lilly Schilling Foundation (to U. Dirnagl) is gratefully acknowledged.


   FOOTNOTES
 

Address for reprint requests and other correspondence: J. P. Dreier, Dept. of Neurology, Humboldt-Universität, Schumannstrasse 20/21, 10117 Berlin, Germany (E-mail: jens.dreier{at}charite.de).

The costs of publication of this article were defrayed in part by the payment of page charges. The article must therefore be hereby marked "advertisement" in accordance with 18 U.S.C. Section 1734 solely to indicate this fact.


   REFERENCES
TOP
 ABSTRACT
 MATERIALS AND METHODS
 RESULTS
 DISCUSSION
 REFERENCES
 

  1. Aitken PG, Tombaugh GC, Turner DA, and Somjen GG. Similar propagation of SD and hypoxic SD-like depolarization in rat hippocampus recorded optically and electrically. J Neurophysiol 80: 1514–1521, 1998.
  2. Basarsky TA, Duffy SN, Andrew RD, and MacVicar BA. Imaging spreading depression and associated intracellular calcium waves in brain slices. J Neurosci 18: 7189–7199, 1998.
  3. Blomstrand F, Giaume C, Hansson E, and Rönnbäck L. Distinct pharmacological properties of ET-1 and ET-3 on astroglial gap junctions and Ca2+ signaling. Am J Physiol Cell Physiol 277: C616–C627, 1999.
  4. Boillot A, Vallet B, Marty J, Auclerc A, and Barale F. Effects of halothane, enflurane and isoflurane on contraction of rat aorta induced by endothelin-1. Br J Anaesth 75: 761–767, 1995.
  5. Bychkov R, Glowinski J, and Giaume C. Sequential and opposite regulation of two outward K+ currents by ET-1 in cultured striatal astrocytes. Am J Physiol Cell Physiol 281: C1373–C1384, 2001.
  6. Bryan RM Jr, You J, Marrelli SP, and Dryer SE. A novel mechanism of vasodilatation in cerebral arteries: activation of tandem pore domain potassium channels. J Cereb Blood Flow Metab 23, Suppl 1: 51, 2003.
  7. Dichgans M, Mayer M, Uttner I, Bruning R, Muller-Hocker J, Rungger G, Ebke M, Klockgether T, and Gasser T. The phenotypic spectrum of CADASIL: clinical findings in 102 cases. Ann Neurol 44: 731–739, 1998.
  8. Dreier JP, Kleeberg J, Petzold G, Priller J, Windmüller O, Orzechowski HD, Lindauer U, Heinemann U, Einhäupl KM, and Dirnagl U. Endothelin-1 potently induces Leão's cortical spreading depression in vivo in the rat: a model for an endothelial trigger of migrainous aura? Brain 125: 102–112, 2002.
  9. Dreier JP, Körner K, Ebert N, Görner A, Rubin I, Back T, Lindauer U, Wolf T, Villringer A, Einhäupl KM, Lauritzen M, and Dirnagl U. Nitric oxide scavenging by haemoglobin or nitric oxide synthase inhibition by N-nitro-L-arginine induce cortical spreading ischaemia when K+ is increased in the subarachnoid space. J Cereb Blood Flow Metab 18: 978–990, 1998.
  10. Dreier JP, Petzold G, Tille K, Lindauer U, Arnold G, Heinemann U, Einhaupl KM, and Dirnagl U. Ischaemia triggered by spreading neuronal activation is inhibited by vasodilators in rats. J Physiol 531: 515–526, 2001.
  11. Duckrow RB. Regional cerebral blood flow during spreading cortical depression in conscious rats. J Cereb Blood Flow Metab 11: 150–154, 1991.
  12. Ehrenreich H, Anderson RW, Ogino Y, Rieckmann P, Costa T, Wood GP, Coligan JE, Kehrl JH, and Fauci AS. Selective autoregulation of endothelins in primary astrocyte cultures: endothelin receptor-mediated potentiation of endothelin-1 secretion. New Biol 3: 135–141, 1991.
  13. Ehrenreich H, Costa T, Clouse KA, Pluta RM, Ogino Y, Coligan JE, and Burd PR. Thrombin is a regulator of astrocytic endothelin-1. Brain Res 600: 201–207, 1993.
  14. Ehrenreich H, Löffler BM, Hasselblatt M, Langen H, Oldenburg J, Subkowski T, Schilling L, and Sirén AL. Endothelin converting enzyme activity in primary rat astrocytes is modulated by endothelin B receptors. Biochem Biophys Res Commun 261: 149–155, 1999.
  15. Fuxe K, Bjelke B, Andbjer B, Grahn H, Rimondini R, and Agnati LF. Endothelin-1 induced lesions of the frontoparietal cortex of the rat. A possible model of focal cortical ischemia. Neuroreport 8: 2623–2639, 1997.
  16. Giaume C, Cordier J, and Glowinski J. Endothelins inhibit junctional permeability in cultured mouse astrocytes. Eur J Neurosci 4: 877–881, 1992.
  17. Giaume C, Tabernero A, and Medina JM. Metabolic trafficking through astrocytic gap junctions. Glia 21: 114–123, 1997.
  18. Giaume C and Venance L. Intercellular calcium signaling and gap junctional communication in astrocytes. Glia 24: 50–64, 1998.
  19. Görlach C, Benyo Z, and Wahl M. Endothelin-1-induced contraction in cerebral vessels mediated by phospholipase C/protein kinase C cascade. Kidney Int 54, Suppl 67: 224–225, 1998.
  20. Grafstein B. Mechanism of spreading cortical depression. J Neurophysiol 19: 154–171, 1956.
  21. Griendling KK, Tsuda T, and Alexander RW. Endothelin stimulates diacylglycerol accumulation and activates protein kinase C in cultured vascular smooth muscle cells. J Biol Chem 264: 8237–8240, 1989.
  22. Guibert C and Beech DJ. Positive and negative coupling of the endothelin ETA receptor to Ca2+-permeable channels in rabbit cerebral cortex arterioles. J Physiol 514: 843–856, 1999.
  23. Harder DR, Alkayed NJ, Lange AR, Gebremedhin D, and Roman RJ. Functional hyperemia in the brain. Hypothesis for astrocyte-derived vasodilator metabolites. Stroke 28: 229–234, 1998.
  24. Hasselblatt M, Kamrowski-Kruck H, Jensen N, Schilling L, Kratzin H, Siren AL, and Ehrenreich H. ETA and ETB receptor antagonists synergistically increase extracellular endothelin-1 levels in primary rat astrocyte cultures. Brain Res 785: 253–261, 1998.
  25. Hasselblatt M, Lewczuk P, Löffler BM, Kamrowski-Kruck H, Von Ahsen N, Sirén AL, and Ehrenreich H. Role of astrocytic ETB receptor in the regulation of extracellular endothelin-1 during hypoxia. Glia 34: 18–26, 2001.
  26. Hori S, Komatsu Y, Shigemoto R, Mizuno N, and Nakanishi S. Distinct tissue distribution and cellular localization of two messenger ribonucleic acids encoding different subtypes of rat endothelin receptors. Endocrinology 130: 1885–1895, 1992.
  27. Ihara M, Noguchi K, Saeki T, Fukuroda T, Tsuchida S, Kimura S, Fukami T, Ishikawa K, Nishikibe M, and Yano M. Biological profiles of highly potent novel endothelin antagonists selective for the ETA receptor. Life Sci 50: 247–255, 1992.
  28. Innocenti B, Parpura V, and Haydon PG. Imaging extracellular waves of glutamate during calcium signaling in cultured astrocytes. J Neurosci 20: 1800–1808, 2000.
  29. Ishikawa K, Ihara M, Noguchi K, Mase T, Mino N, Saeki T, Fukuroda T, Fukami T, Ozaki S, Nagase T, Nishikibe M, and Yano M. Biochemical and pharmacological profile of a potent and selective endothelin B-receptor antagonist, BQ-788. Proc Natl Acad Sci USA 91: 4892–4896, 1994.
  30. Jamme I, Petit E, Gerbi A, Maixent JM, MacKenzie ET, and Nouvelot A. Changes in ouabain affinity of Na+,K+-ATPase during focal cerebral ischaemia in the mouse. Brain Res 774: 123–30, 1997.
  31. Jensen N, Hasselblatt M, Siren AL, Schilling L, Schmidt M, and Ehrenreich H. ETA and ETB specific ligands synergistically antagonize endothelin-1 binding to an atypical endothelin receptor in primary rat astrocytes. J Neurochem 70: 473–482, 1998.
  32. Kaube H, Knight YE, Storer RJ, Hoskin KL, May A, and Goadsby PJ. Vasodilator agents and supracollicular transection fail to inhibit cortical spreading depression in the cat. Cephalalgia 19: 592–597, 1999.
  33. Kedzierski RM and Yanagisawa M. Endothelin system: the double-edged sword in health and disease. Annu Rev Pharmacol Toxicol 41: 851–876, 2001.
  34. Koizumi S, Kataoka Y, Niwa M, Yamashita K, Taniyama K, and Kudo Y. Endothelin increased [Ca2+]i in cultured neurones and slices of rat hippocampus. Neuroreport 5: 1077–1080, 1994.
  35. Kunkler PE and Kraig RP. Calcium waves precede electrophysiological changes of spreading depression in hippocampal cultures. J Neurosci 18: 3416–3425, 1998.
  36. Kuwaki T, Kurihara H, Cao WH, Kurihara Y, Unekawa M, Yazaki Y, and Kumada M. Physiological role of brain endothelin in the central autonomic control: from neuron to knockout mouse. Prog Neurobiol 51: 545–579, 1997.
  37. Largo C, Cuevas P, Somjen GG, Martin del Rio R, and Herreras O. The effect of depressing glial function in rat brain in situ on ion homeostasis, synaptic transmission, and neuron survival. J Neurosci 16: 1219–1229, 1996.
  38. Lazarini F, Strosberg AD, Couraud PO, and Cazaubon SM. Coupling of ETB endothelin receptor to mitogen-activated protein kinase stimulation and DNA synthesis in primary cultures of rat astrocytes. J Neurochem 66: 459–465, 1996.
  39. Lauritzen M, Hansen AJ, Kronborg D, and Wieloch T. Cortical spreading depression is associated with arachidonic acid accumulation and preservation of energy charge. J Cereb Blood Flow Metab 10: 115–122, 1990.
  40. Leão AAP. Spreading depression of activity in the cerebral cortex. J Neurophysiol 7: 359–390, 1944.
  41. Leonova J, Thorleif T, Åberg ND, Eriksson PS, Rönnbäck L, and Hansson E. Endothelin-1 decreases glutamate uptake in primary cultured rat astrocytes. Am J Physiol Cell Physiol 281: C1495–C1503, 2001.
  42. Martins-Ferreira H, Nedergaard M, and Nicholson C. Perspectives on spreading depression. Brain Res Brain Res Rev 32: 215–234, 2000.
  43. Müller M and Somjen GG. Na+ and K+ concentrations, extra- and intracellular voltages, and the effect of TTX in hypoxic rat hippocampal slices. J Neurophysiol 83: 735–45, 2000.
  44. Narushima I, Kita T, Kubo K, Yonetani Y, Momochi C, Yoshikawa I, Shimada K, and Nakashima T. Contribution of endothelin-1 to disruption of blood-brain barrier permeability in dogs. Naunyn Schmiedebergs Arch Pharmacol 360: 639–645, 1999.
  45. Nedergaard M. Direct signaling from astrocytes to neurons in cultures of mammalian brain cells. Science 263: 1768–1771, 1994.
  46. Nedergaard M, Cooper AJ, and Goldman SA. Gap junctions are required for the propagation of spreading depression. J Neurobiol 28: 433–444, 1995.
  47. Nedergaard M and Hansen AJ. Characterization of cortical depolarizations evoked in focal cerebral ischemia. J Cereb Blood Flow Metab 13: 568–574, 1993.
  48. Patel TR, McAuley MA, and McCulloch J. Endothelin receptor mediated constriction and dilatation in feline cerebral resistance arterioles in vivo. Eur J Pharmacol 307: 41–48, 1996.
  49. Pellerin L and Magistretti PJ. Glutamate uptake into astrocytes stimulates aerobic glycolysis: a mechanism coupling neuronal activity to glucose utilization. Proc Natl Acad Sci USA 91: 10625–10629, 1994.
  50. Petzold GC, Einhäupl KM, Dirnagl U, and Dreier JP. Ischemia triggered by spreading neuronal activation is induced by endothelin-1 and hemoglobin in the subarachnoid space. Ann Neurol 54: 591–598, 2003.
  51. Saito R, Graf R, Hubel K, Taguchi J, Rosner G, Fujita T, and Heiss WD. Halothane, but not alpha-chloralose, blocks potassium-evoked cortical spreading depression in cats. Brain Res 699: 109–115, 1995.
  52. Sasaki Y, Takimoto M, Oda K, Fruh T, Takai M, Okada T, and Hori S. Endothelin evokes efflux of glutamate in cultures of rat astrocytes. J Neurochem 68: 2194–2200, 1997.
  53. Seiffert E, Dreier JP, Heinemann U, and Friedman A. Electrophysiological responses to cortical blood-brain-barrier disruption (Abstract). Soc Neurosci Abstr 533.24: 8938, 2003.
  54. Shihara M, Hirooka Y, Hori N, Matsuo I, Tagawa T, Suzuki S, Akaike N, and Takeshita A. Endothelin-1 increases the neuronal activity and augments the responses to glutamate in the NTS. Am J Physiol Regul Integr Comp Physiol 275: R658–R665, 1998.
  55. Smith SJ. Neural signalling. Neuromodulatory astrocytes. Curr Biol 4: 807–810, 1994.
  56. Somjen GG. Mechanisms of spreading depression and hypoxic spreading depression-like depolarization. Physiol Rev 81: 1065–1096, 2001.
  57. Stanimirovic DB, Bertrand N, McCarron R, Uematsu S, and Spatz M. Arachidonic acid release and permeability changes induced by endothelins in human cerebromicrovascular endothelium. Acta Neurochir Suppl (Wien) 60: 71–75, 1994.
  58. Tabernero A, Giaume C, and Medina JM. Endothelin-1 regulates glucose utilization in cultured astrocytes by controlling intercellular communication through gap junctions. Glia 16: 187–195, 1996.
  59. Touzani O, Galbraith S, Siegl P, and McCulloch J. Endothelin-B receptors in cerebral resistance arterioles and their functional significance after focal cerebral ischaemia in cats. J Cereb Blood Flow Metab 17: 1157–1165, 1997.
  60. Tzourio C, El Amrani M, Poirier O, Nicaud V, Bousser MG, and Alperovitch A. Association between migraine and endothelin type A receptor (ETA-231 A/G) gene polymorphism. Neurology 56: 1273–1277, 2001.
  61. Vahedi K, Massin P, Guichard JP, Miocque S, Polivka M, Goutieres F, Dress D, Chapon F, Ruchoux MM, Riant F, Joutel A, Gaudric A, Bousser MG, and Tournier-Lasserve E. Hereditary infantile hemiparesis, retinal arteriolar tortuosity, and leukoencephalopathy. Neurology 60: 57–63, 2003.
  62. Van Harreveld A and Fifkova E. Mechanisms involved in spreading depression. J Neurobiol 4: 375–387, 1973.
  63. Venance L, Premont J, Glowinski J, and Giaume C. Gap junctional communication and pharmacological heterogeneity in astrocytes cultured from the rat striatum. J Physiol 510: 429–440, 1998.
  64. Venance L, Stella N, Glowinski J, and Giaume C. Mechanism involved in initiation and propagation of receptor-induced intercellular calcium signaling in cultured rat astrocytes. J Neurosci 17: 1981–1992, 1997.
  65. Vilagi I, Klapka N, and Luhmann HJ. Optical recording of spreading depression in rat neocortical slices. Brain Res 898: 288–296, 2001.
  66. Zhou QL, Davar G, and Strichartz G. Endothelin-1 (ET-1) selectively enhances the activation gating of slowly inactivating tetrodotoxin-resistant sodium currents in rat sensory neurons: a mechanism for the pain-inducing actions of ET-1. J Neurosci 22: 6325–6330, 2002.
  67. Zhou QL, Strichartz G, and Davar G. Endothelin-1 activates ETA receptors to increase intracellular calcium in model nociceptors. Neuroreport 12: 3853–3857, 2001.



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