Protease activated receptor 1-induced glutamate release in cultured astrocytes is mediated by Bestrophin-1 channel but not by vesicular exocytosis
© Oh et al.; licensee BioMed Central Ltd. 2012
Received: 28 September 2012
Accepted: 9 October 2012
Published: 12 October 2012
Glutamate is the major transmitter that mediates the principal form of excitatory synaptic transmission in the brain. It has been well established that glutamate is released via Ca2+-dependent exocytosis of glutamate-containing vesicles in neurons. However, whether astrocytes exocytose to release glutamate under physiological condition is still unclear.
We report a novel form of glutamate release in astrocytes via the recently characterized Ca2+-activated anion channel, Bestrophin-1 (Best1) by Ca2+ dependent mechanism through the channel pore. We demonstrate that upon activation of protease activated receptor 1 (PAR1), an increase in intracellular Ca2+ concentration leads to an opening of Best1 channels and subsequent release of glutamate in cultured astrocytes.
These results provide strong molecular evidence for potential astrocyte-neuron interaction via Best1-mediated glutamate release.
KeywordsAstrocyte Bestrophin-1 Glutamate
Astrocytes and neurons are intimate partners in the brain. Astrocytes respond to neuronal activity by an increase in intracellular Ca2+ ([Ca2+i) [1, 2]. The synaptically released neurotransmitters such as glutamate and ATP activate corresponding Gαq protein-coupled receptors expressed in astrocytes, resulting in increase in [Ca2+i and Ca2+-dependent release of gliotransmitters from astrocytes [2, 3]. These gliotransmitters in turn influence the neuronal excitability and synaptic activities [3–8].
At the heart of this neuron-glia interaction there is glutamate, which is released from neurons by synaptic vesicles to mediate neuron-to-glia communication and from astrocytes by various Ca2+-dependent mechanisms to mediate glia-to-neuron communication [9, 10]. Therefore, understanding how astrocytes release glutamate in Ca2+-dependent manner and how astrocytically-released glutamate regulates neuronal synaptic activity has been a major challenge. One line of accumulating evidence supports that astrocytes release glutamate by Ca2+- and SNARE-dependent exocytosis mechanism , although this mechanism has been recently challenged . It has been reported that glutamate released by SNARE-dependent mechanism regulates hippocampal synapse between perforant path afferents and granule cells  or Schaffer Collateral afferent and CA1 pyramidal neurons  through N-methyl-D-aspartic acid receptor (NMDAR) activation. Yet, astrocytes also express a combination of anion-permeable channels to move Cl- and large anions such as glutamate across membranes in response to specific physiological stimulations [14, 15], raising the possibility that astrocytes have a multiple glutamate release mechanisms. Although astrocytes under physiological conditions appear to possess a Ca2+- and anion channel-dependent glutamate release mechanism [10, 16], until now this idea has not been directly demonstrated due to the lack of molecular evidence.
Bestrophin is the gene identified as the gene responsible for Best's vitelliform macular dystrophy and has been shown to encode a functional Ca2+-activated anion channel (CAAC) in nonneuronal tissue and peripheral neurons . This Bestrophin-1 channel (Best1) is directly activated by submicromolar intracellular Ca2+ concentration and has an anion selective pore with single channel activities [17–24]. Recently, we have discovered that astrocytes express CAAC and that Best1 encodes most of the CAAC in astrocytes . This astrocytic CAAC showed a considerable permeability to large anions such as isethionate and glutamate . In addition, we have recently demonstrated that Best1 channel mediates tonic GABA release from cerebellar glia by a direct permeation . Therefore, we hypothesized that Best1 is the molecular identity of Ca2+-dependent anion channel that mediates glutamate release from astrocytes. Here we tested whether Best1 is an alternative Ca2+-dependent glutamate release mechanism in cultured astrocytes. To stimulate astrocytes more physiologically, we activated endogenous GPCRs by application of TFLLR  a selective peptide agonist of the protease activated receptor 1 (PAR1). We demonstrate that PAR1-induced glutamate release is mediated not by conventional vesicular exocytosis but by an activation of glutamate permeable anion channel Best1 in cultured astrocytes.
PAR1-induced glutamate release is mediated by CAAC
Best1 mediates a Ca2+-dependent glutamate release in cultured astrocytes
PAR1 induced glutamate release is not due to vesicular release
In this study we report the direct evidence of anion channel-mediated glutamate release mechanism. We provide a series of evidence for Ca2+-activated, Best1-mediated glutamate release from astrocytes. For example, the selective gene silencing of astrocytic Best1 channels significantly reduced GPCR-induced and Ca2+-dependent glutamate release from astrocytes as measured by HPLC detection of glutamate from cultured astrocytes (Figure 3), and by FRET glutamate sensor in cultured astrocytes (Figure 4). The FRET based glutamate sensor has been well-characterized in the previous report . In that report it has been demonstrated that FRET change is quite specific for glutamate because the sensor shows binding kinetics and high selectivity toward glutamate with no apparent change in ratio with APV, NBQX, NMDA, KA, AMPA, etc. . We performed a calibration experiment by measuring glutamate EC50 in our imaging system and experimental conditions. Our calibration results showed that the FRET-based glutamate sensor in cultured astrocyte can be useful in detecting micromolar and submicromolar concentrations of released extracellular glutamate from a single astrocyte.
Until now, it has been proposed that glutamate could be released from astrocytes through multiple routes, including Ca2+- and SNARE-dependent vesicular exocytosis, the reversal action of glutamate transporters, transportation by cystine-glutamate antiporter, and permeation through channels or receptors, such as P2X7 receptor, volume regulated anion channel (VRAC), or gap junction hemichannel . Among these, the molecular mechanism of Ca2+-dependent glutamate release has been extensively studied mainly because the generation of astrocytic Ca2+ transient responding to neuronal activity is one of the most important physiological readout of neural activity [3, 5, 7, 10]. Numerous studies have proposed the SNARE-dependent exocytosis of glutamate as a potential route for astrocytic Ca2+-dependent glutamate release. These studies demonstrated that astrocytic glutamate release was sensitive to exocytosis blockers or the expression of the essential machineries for regulating Ca2+-dependent exocytosis . In addition to the vesicular mechanism, there is multiple lines of evidence suggesting that astrocytes express a Ca2+-dependent but non-vesicular glutamate release machinery . Despite its unclear molecular identity, it has been reported that an increase in Ca2+ by GPCR activation induces glutamate release from astrocytes through osmolyte-permeable anion channels [10, 28], which are activated by intracellular Ca2+ or increase in cell volume . In our previous reports, we observed that Best1-mediated Ca2+-activated anion current could be induced by a host of GPCR agonists such as mGluR1/5, P2Y, B2, S1P, and LPAR in astrocytes , and that activation of those receptors elicits Ca2+-dependent glutamate release . Finally, Best1 was demonstrated to be permeable to GABA and mediate tonic GABA release in cerebellar glial cells . Recent study showed that GABA is abundant in cerebellar glial cells to be released tonically via Best1 to cause tonic inhibition . However, in hippocampus, GABA is not present in glial cells; rather, Best1 might release glutamate near synapse. Therefore, it is plausible that Best1, at least in part, could be the downstream target of various Gq-coupled GPCRs that signal through intracellular Ca2+ to release glutamate in hippocampal astrocytes.
In addition to Best1 channel, other anion channels might participate in anion channel-mediated glutamate release as previously suggested, such as Ca2+-induced but volume regulated osmolyte-permeable channels . In fact, there are several studies showing that bestrophin channel could be opened by both cytosolic Ca2+ and cell volume increase [17, 35], raising a possibility that Best1-mediated glutamate release is also triggered by Ca2+-dependent cell swelling and subsequent activation of VRAC. However, in our previous study we demonstrated that PAR-1 activation does not induce significant swelling  indicating that Ca2+ directly initiates Best1 channel-mediated glutamate release from astrocytes. The PAR1-induced astrocytic glutamate release was not completely inhibited by Best1 knock-down (Figure 4). Still, vesicular release mechanism was not involved because Best1 silencing did not affect the expression level of known genes involved in vesicular release (Figure 5A) and glutamate release from astrocytes was not reduced by treatment with Conconomycin A or Tetanus toxin (Figure 5B). There is a possibility that other ion channels that are independent of Best1 channel might participate in PAR1-induced glutamate release from astrocytes.
We utilized the native GPCR, PAR1, which has been extensively used in numerous studies to selectively activate astrocytes. Even though PAR1 is expressed in a subset of dentate granule cells , PAR1 has been shown to be expressed exclusively in astrocytes in human and rodent CA1 hippocampus [7, 38, 39], as well as in the nucleus of solitary tract  to mediate neuron-glia interaction. Therefore, the source of PAR1-induced glutamate is most likely astrocyte, as a direct consequence of increase [Ca2+i. Although there is no direct evidence of how PAR1 is activated in the physiological situation up to now, the recent study demonstrated that tPA-plasmin pathway is an endogenous PAR1 agonist , suggesting that physiological PAR1 activation is initiated by the activation of tPA-plasmin pathway in physiological condition such as synaptic plasticity [42, 43].
In summary, we reveal a novel anion channel-mediated glutamate release mechanism in cultured astrocytes. The ideas and tools developed in this study should prove to be helpful in understanding the physiological role of glutamate release mechanism and its functional significances.
Primary astrocyte culture
Cell culture of mouse astrocytes was performed as previously described . The cerebral cortex from P0 ~ P3 postnatal mice was dissected free of adherent meninges, minced and dissociated into single cell suspension by trituration. Dissociated cells were plated onto 12 mm glass coverslips coated with 0.1 mg/ml poly D-lysine. Cells were grown in DMEM supplemented with 25 mM glucose, 10% heat-inactivated horse serum, 10% heat-inactivated fetal bovine serum, 2 mM glutamine, and 1000 units ml-1 penicillin-streptomycin. Cultures were maintained at 37°C in humidified 5% CO2-containing atmosphere.
Glutamate FRET imaging
In FRET-based glutamate imaging experiments, pDisplay- GluSnFR vector  was electroporated alone or with pSicoR-scrambled-shRNA or pSicoR-Best1-shRNA vector into cultured astrocytes (MicroPorator; Digital Bio, Korea). After 48 ~ 72 hour expression, FRET imaging was performed under a microscope (BX50WI; Olympus) equipped with xenon lamp with 436/20 excitation filter (D436/20x filter; Chroma). The emission beam was split with a DualView (Optical Insights) with a CFP/YFP filter set (OI-05-EX), recorded by EM-CCD camera (ANDOR IXON). Imaging Workbench software (INDEC BioSystems) was used for image acquisition and offline image analysis. TFLLR puff (TFLLR-NH2; Peptron, Korea; 500 μM) was made by using picospritzer-assisted positive pressure (~100 ms). The amount of released extracellular glutamate was described as ratio between the emission intensity of CFP and YFP (CFP/YFP), which was divided by baseline CFP/YFP ratio (relative CFP/YFP ratio).
Radioactivity glutamate release assay
In vitro glutamate assay using 3H-labelled glutamate was performed as described previously . Astrocytes were loaded with 0.5 μm l-3H]glutamate for 60 min by adding 1 μm of 1 mCi ml−1 l-3H]glutamate stock solution to 2 ml of culture medium. The cultures were preincubated for 30 min with 1 mm amino-oxyacetic acid and 0.5 mm methionine sulfoximine before adding 3H]glutamate, and during the loading to inhibit the metabolism of glutamate to glutamine and other metabolites . Cells were washed with external solution 3 times. In some experiments, the external solution was supplemented with 50 μm l-transpyrrolidine-2,4-dicarboxylic acid (trans-PDC) to block glutamate transporter, a maximally effective concentration (6× IC50 of 4–8 μm; ) that is well below that suggested to stimulate heteroexchange (0.2 mm; [46, 47]). Agonists were added to external solution for 6 min and the experiment was terminated by collection of the solution. Each experimental run included the control condition in which no agonist was added. Six replicates were obtained for each drug condition. For analysis, the average radioactivity count was obtained from six replicates for each condition and compared to the average of control.
HPLC analysis for glutamate release
The Cortical primary astrocytes were cultured in 60 mm dishes for HPLC analysis. TFLLR (30 μM) was used to induce glutamate. Prior to TFLLR treatment, astrocytes were washed with PBS three times. For gene silencing experiment, Lentivirus containing Scrambled or Best1-shRNA was treated to cells and incubated for 48 hrs. The amino acid content was derivatized with o-phthaldialdehyde (OPA) and detected using UV (DAD) detection . The OPA derivatized samples by programmed autosampler were injected on Zorbax Eclipse Plus C18 column with detection at 338 nm (a reference = 390 nm). Mobile phase A was 40 mM Na2HPO4 pH 7.8, and B was acetonitrile/methanol/water (45:45:10, v/v/v). The flow rate was 2 mL/min with a gradient condition that allowed for 1.9 min at 0% B and raised to 26% B at a 12.5 min-step. Then washing at 100% B and equilibration at 0% B was performed in a total retention time of 15 min. Reagents of OPA derivatization and all equipments for HPLC analysis were obtained from Agilent Technologies.
Lentivirus with Best1-shRNA and Best1 mutagenesis
Best1-shRNA and lentivirus production were performed as previously described (, Virus facility, KIST). Best1 shRNA-insensitive pore mutant (Best1-shRNA insens W93C) was generated by using PCR-based site-directed mutagenesis kit (Stratagene, Cedar Creek, TX, USA).
The extracellular recording solution for perforated patch clamp recording was comprised of (in mM) 150 NaCl, 10 HEPES, 3 KCl, 2 CaCl2, 2 MgCl2, 5.5 glucose, at pH 7.3. The internal solution contained 25 μg/ml gramicidin D and (in mM) 75 Cs2SO4, 10 NaCl, 0.1 CaCl2, and 10 HEPES, at pH 7.1. Pipette resistances ranged from 5 to 8 MΩ. It took 20 to 30 min to achieve acceptable perforation, with final series resistances ranging from 15 to 40 MΩ. Current voltage curves were established by applying 100- , 200-, or 1000 ms duration voltage ramps from –100 to +100 mV. Data were acquired by an Axopatch 200A amplifier controlled by Clampex 9.2 via Digidata 1322A data acquisition system (Axon Instruments, Union City, CA, USA). Experiments were conducted at room temperature (20 ~ 24°C).
Total RNA was prepared from cultured astrocyte from postnatal day 0–3 mice using Trizol reagent (Invitrogen). cDNA was synthesized using Super Script III reverse transcriptase (Invitrogen). The reverse transcription (RT)-PCR primers used to check expression of Best1, Syt4 (Synaptotagmin4), Munc18-1, Vamp2 (Vesicle-associated membrane protein 2) GAPDH and glial fibrillary acidic protein (GFAP) were as followings
; Best1 forward, 5’-AGGACGATGATGATTTTGAG- 3’
; Best1 reverse, 5’-CTTTCTGGTTTTTCTGGTTG- 3’
; Syt4 forward, 5’-AGGCCAATTCCCCTGAGAGC- 3’
; Syt4 reverse, 5’-ACCGCTTCCTTCTGCTGTGG- 3’
; Munc18-1 forward, 5’-ACTCCGCTGACTCTTTCCAA- 3’
; Munc18-1 reverse, 5’-GTCGGCTTTATAGGCATCCA- 3’
; Vamp2 forward, 5’-GTCACTGCCTCTGCCAAGTC- 3’
; Vamp2 reverse, 5’-GGCAGACTCCTCAGGGATTT- 3’
; GAPDH forward, 5’-AGCTGAACGGGAAGCTCACT- 3’
; GAPDH reverse, 5’-TGCTGTAGCCAAATTCGTTG- 3’
; GFAP forward, 5’-AGAACAACCTGGCTGCGTAT-3’
; GFAP reverse, 5’-CGGCGATAGTCGTTAGCTTC-3’
This work was supported by the National Research Foundation of Korea (NRF) grant funded by the Korea government (MEST) (No. 314-2008-1-C00341).
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