Activation of protease activated receptor 1 increases the excitability of the dentate granule neurons of hippocampus
© Han et al; licensee BioMed Central Ltd. 2011
Received: 13 June 2011
Accepted: 10 August 2011
Published: 10 August 2011
Protease activated receptor-1 (PAR1) is expressed in multiple cell types in the CNS, with the most prominent expression in glial cells. PAR1 activation enhances excitatory synaptic transmission secondary to the release of glutamate from astrocytes following activation of astrocytically-expressed PAR1. In addition, PAR1 activation exacerbates neuronal damage in multiple in vivo models of brain injury in a manner that is dependent on NMDA receptors. In the hippocampal formation, PAR1 mRNA appears to be expressed by a subset of neurons, including granule cells in the dentate gyrus. In this study we investigate the role of PAR activation in controlling neuronal excitability of dentate granule cells. We confirm that PAR1 protein is expressed in neurons of the dentate cell body layer as well as in astrocytes throughout the dentate. Activation of PAR1 receptors by the selective peptide agonist TFLLR increased the intracellular Ca2+ concentration in a subset of acutely dissociated dentate neurons as well as non-neuronal cells. Bath application of TFLLR in acute hippocampal slices depolarized the dentate gyrus, including the hilar region in wild type but not in the PAR1-/- mice. PAR1 activation increased the frequency of action potential generation in a subset of dentate granule neurons; cells in which PAR1 activation triggered action potentials showed a significant depolarization. The activation of PAR1 by thrombin increased the amplitude of NMDA receptor-mediated component of EPSPs. These data suggest that activation of PAR1 during normal function or pathological conditions, such as during ischemia or hemorrhage, can increase the excitability of dentate granule cells.
Protease activated receptor 1 (PAR1) is a G-protein coupled receptor that is best known for its role in coagulation and homeostasis [1–3]. PAR-1 is activated when serine proteases such as thrombin or plasmin cleave the N-terminus at Arg41, revealing a new N-terminus that acts as a tethered ligand to activate receptor signaling [4, 5]. PAR-1 signals through multiple G-proteins, including Gi, Gq, and G12/13 [5–7], and is highly expressed in astrocytes throughout the CNS [8–10], and differentially expressed in neuronal subpopulations in discrete regions, including granule cell layer of dentate gyrus [8, 11, 12]. Activation of PAR1 leads to profound changes in astrocyte function, such as the proliferation [13–15] that underlies glial scar formation in response to penetrating head wound . Activation of astrocytic PAR1 also triggers the release of glutamate and subsequent potentiation of neuronal NMDA receptors secondary to depolarization-induced relief of Mg2+ block [9, 16, 17]. In the present study, we have investigated the functional expression of PAR1 in granule cells of the dentate gyrus. We show that PAR1 activation leads to granule cell depolarization and potentiation of synaptically-activated NMDA receptor function.
PAR1 expression in dentate granule cells
PAR1 activation in acutely dissociated dentate neurons increases intracellular [Ca2+]
PAR1 activation depolarizes dentate gyrus in wild type but not in PAR1 -/- mice
PAR1 activation triggers action potential generation in a subset of dentate granule cells
PAR1 activation increases NMDA receptor-mediated EPSPs in dentate granule cells
We initially measured non-NMDA receptor-mediated EPSPs in the presence of bicuculline to block GABAA receptors. We subsequently supplemented the recording solution with 10 μM CNQX and reduced the extracellular Mg2+ to 5 μM to isolate the NMDA receptor component of the evoked EPSPs. Following recording of EPSPs during a control period, we applied 30 nM thrombin to activate PAR1 to slices while recording the pharmacologically-isolated NMDA receptor-mediated component of the evoked EPSP. We found that PAR1 activation by thrombin increased the amplitude of the NMDA receptor-mediated EPSP (Figure 5B, D; 137 ± 14% of control; p < 0.009, paired t-test; n = 12), whereas the amplitude of the AMPA receptor-mediated EPSP was only minimally altered by thrombin (data not shown; 113 ± 5% of control, p < 0.03, paired t-test; n = 9).
To confirm the result we obtained imaging voltage-sensitive dye imaging, we performed field potential recordings in the dentate molecular layer of hippocampal slices in response to stimulation of the perforant path. To isolate NMDA receptor-mediated field EPSP, 2 μM CNQX was added and concentration of Mg2+ was reduced to 0.1 mM. PAR1 activation by 30 nM thrombin significantly increased the amplitude of field EPSPs compared to slices recorded in ACSF alone (Figure 5C~D; p < 0.05, unpaired t-test; n = 12-13). This result is consistent with data from voltage-dye recordings, and confirms that PAR1 activation can enhance the NMDA component of excitatory transmission at the perforant path-granule cell synapse.
The most important finding of this study is that PAR1 activation induces both an increase in intracellular Ca2+ and depolarization accompanied by spike firing in a subset of dentate granule neurons. In addition, PAR1 activation enhances the NMDA receptor component of the perforant path-granule cell EPSP in the dentate gyrus. The sum of these actions will be to enhance both the excitability of the dentate gyrus and the excitatory drive reaching the hippocampus. These data provide the first description of the functional effects of PAR1 activation on the dentate granule neurons.
Previous immunohistochemical studies have shown that PAR1 protein is expressed primarily in human astrocytes of white and gray matter in the cortex, hippocampus, caudate, putamen, and cerebellum . By contrast, larger pyramidal neurons of the hippocampus and cortex show only modest PAR1 immunoreactivity in human brain . Our immunocytochemical data indicate that PAR1 is also expressed in the dentate granule neurons, consistent with in situ hybridization data suggesting PAR1 expression in dentate gyrus [11, 12]. Moreover, the immunohistochemical data are consistent with electrophysiological recordings from hippocampal slices, in which a subset of granule neurons show functional responses to PAR1 activation.
PAR1 activation and Ca2+ increase
The PAR1 receptor is functionally linked to multiple G-proteins, including Gαq/11. PAR1 activation leads to a cleavage of PIP2 by phospholipase (PLC) to generate 1, 2-diacylglycerol (DAG) and inositol 1, 4, 5 triphosphate (IP3). Activation of IP3 receptors increases intracellular Ca2+. Thus, the observation that a subset of NMDA-responsive acutely dissociated cells shows an increase in intracellular Ca2+ in response to PAR1 activation suggests that dentate neurons express PAR1 that is functionally coupled to Gαq/11. These data are consistent with previous study of cultured neurons from the hippocampal formation, that included the dentate gyrus . In addition, data obtained from acutely dissociated cells studied here strongly suggest that PAR1 is functionally expressed in intact tissue, since the acute dissociation protocol eliminates potential confounds associated with culture conditions that could alter PAR1 expression. However, neuronal data from slice recordings showing strong depolarization following PAR1 activation raises the possibility that some of the increase in intracellular Ca2+ we observe may have been supplemented by transmembrane flux through voltage gated Ca2+ channels that could be activated by neuronal depolarization. There is another possible mechanism of Ca2+ increase by PAR1 activation. It has been reported that Ca2+ influx from extracellular region elicits Ca2+ induced Ca2+ release (CICR) through ryanodine receptors in the dentate gyrus . Therefore, Ca2+ induced Ca2+ release may contribute to PAR1 induced Ca2+ increase in the dentate gyrus.
PAR1 activation and neuronal excitability
The depolarization of dentate granule cells by PAR1 activation could reflect the sum of multiple mechanisms. It has been suggested that activation of the H1 receptor, which is linked to Gαq signalling pathways, induces neuronal depolarization by blocking background K+ channel [30–32]. PAR1 could engage this same pathway in a subset of granule cells to lead to modification of K+ channel activity and subsequent depolarization. In addition, PAR1-mediated increases in intraneuronal Ca2+ could enhance the activation of a non-selective cation current, such as those mediated by TRP channels . We and others have also described a mechanism by which PAR1 activation in astrocytes triggers release of ~1 μM glutamate into the extracellular space [9, 17, 34]. This astrocyte-derived glutamate release has also been shown to activate NMDA receptors on neurons, which can lead to neuronal depolarization. Thus, multiple possible mechanisms exist by which PAR1-mediated increases in granule cell intracellular Ca2+ could depolarize these neurons.
PAR1 activation increases the synaptically-evoked NMDA receptor-mediated component of the EPSP produced by perforant path stimulation. The PAR1-triggered enhancement in the evoked EPSP was blocked by APV and higher Mg2+ concentration (data not shown), suggesting that depolarization-induced relief of Mg2+ blockade may be required for thrombin-induced potentiation of NMDAR. Several previous studies have described a new mechanism by which astrocytic PAR1 activation can evoke Ca2+-dependent glutamate release from astrocyte that subsequently controls synaptic NMDA receptor function in neurons [9, 17]. Furthermore, D-seine, an NMDAR glycine site agonist, released from astrocyte in a Ca2+ dependent manner can also regulate the function of NMDA receptor . The depolarization of dentate granule neurons will reduce Mg2+ blockade of NMDA receptor, resulting in an apparent enhancement of the synaptic NMDA receptor response in the presence of Mg2+. Our data are consistent with the idea that this mechanism is operational in the dentate gyrus.
In addition PAR1 activation could also lead to the generation of lysophosphatidic acid and arachidonic acid, a mechanism that previously has been described in platelets and endothelial cells . Both of these lipid signaling molecules are highly mobile and capable of mediating intercellular signaling. Although it is not yet known whether PAR1 activation in dentate gyrus can trigger formation of these lipids, release of lysophosphatidic acid or arachidonic acid could potentially play a role in the effects described here. Whereas arachidonic acid can directly potentiate neuronal NMDA receptor function , lysophosphatidic acid has been suggested to enhance NMDA receptor function through depolarization-induced relief of Mg2+ block . Further work is needed to determine the relative contribution of these (and other) mechanism(s) to PAR1-induced depolarization of dentate granule cells.
Function of PAR1 in physiological and pathological conditions
The physiological role of PAR1 receptors in normal synaptic transmission has not been extensively investigated. Interestingly, tissue plasminogen activator (tPA), which is known to convert plasminogen to plasmin, can influence long-term potentiation, an NMDA receptor-dependent cellular model of learning and memory . Several lines of evidence indicate that plasmin can regulate the function of NMDA receptors through PAR1 activation [34, 40]. Similarly, PAR1 -/- mice show deficiencies in emotional learning, an NMDA receptor-dependent process . Taken together, these results suggest that tPA-activated plasmin could be an endogenous ligand for PAR1 receptor  that leads to PAR1-mediated tuning of NMDA receptor function in a manner relevant for synaptic plasticity and behavior. By potentiating synaptic NMDA receptor, we predict that PAR1 activation would decrease threshold for stimuli needed to trigger changes in synaptic strength. Consistent with this idea, multiple studies have shown that PAR1 activation can influence the threshold for LTP [42, 43]. In addition, sufficient thrombin can enter brain tissue in pathological conditions such as ischemia or hemorrhage and activate PAR1 receptor, which in multiple animal models has been shown to enhance neuronal damage [44–54]. During ischemia, the harmful actions of PAR1 require NMDA receptor function . Our data are consistent with the idea that PAR1 activation in the dentate gyrus can enhance neuronal excitability, which may promote NMDA-receptor mediated excitotoxicity in neurons [43, 45, 56].
Wild type C57Bl/6 mice were deeply anesthetized by 2% avertin (20 μl/g) and transcardially perfused with 4% paraformaldehyde. All procedures involving the use of animals were reviewed and approved by the Emory University IACUC. The brain was isolated, and cut at 30 μm with a cryostat. Sections were blocked in 0.1 M PBS containing 0.3% triton X-100 (Sigma) and 2% serum from species of the secondary antibody for 1 hr. Thrombin receptor goat polyclonal antibody against mouse PAR1 N-terminal (S-19; Santa Cruz; catalog # sc-8204) was applied at 1:20 dilution (S-19) and incubated overnight at 4°C. After overnight incubation, the sections were washed three times in phosphate-buffered saline (PBS) and then incubated in secondary antibody (Alexa 555 donkey anti-'goat IgG; Invitrogen; 1:400) for 2 hr. After three rinses in PBS, the sections were mounted on slide glass. Images were acquired on an Olympus Fluoview FV1000 confocal microscope and analyzed using Image J software.
Adult Sprague-Dawley rats were given a lethal dose of pentobarbital (150 mg/kg) and subsequently transcardially perfused with cold 3% paraformaldehyde (4°C). The brain was subsequently isolated, post-fixed in 3% paraformaldehyde for 24 hrs, cryoprotected in 30% sucrose and 0.1 M phosphate, frozen on dry ice, and cut at 40 μm on a sliding microtome. The sections were washed 6 times (10 min each) in Tris-buffered saline (TBS), and incubated in 3% H2O2 to block endogenous peroxidases. The sections were washed 3 times (10 min each) in TBS plus 0.1% Triton X-100, followed by incubation with the monoclonal WEDE15 PAR1 antibody (5 μg/ml, Immunotech-Coulter; epitope residues 51-64 in exon2, KYEPFWEDEEKNES) in 10% horse serum in TBS overnight at 4°C. The sections were washed 3 times (10 min) in TBS and incubated for 1 hr in biotin-conjugated rat anti-mouse secondary antibody (1:200) in 10% horse serum in TBS plus 0.1% Triton X-100. The sections were washed 3 times (10 min) in TBS and the avidin-biotin complex method was used to detect antigen signal. 3,3'-diamino benzidine tetrachloride was used to visualize the final product. Immunostained sections were mounted on slides and visualized using bright field microscopy; data were obtained from three independent experiments, and showed similar staining patterns. No immunoreactivity could be detected when either the primary or secondary antibody was omitted from the protocol (data not shown). Inclusion of a peptide matching the epitope blocked staining in dentate gyrus (data now shown).
Primary astrocyte culture
Cultured astrocytes were prepared from P0~P3 postnatal mice. The cerebral cortex 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. Astrocyte cultures prepared in this way were confirmed by GFAP staining using anti-GFAP antibody (Millipore; catalog # AB5541; 1:1000)
Adult rat and mouse brain regions were dissected, homogenized in ice cold RIPA buffer (phosphate buffered saline, 1% Igepal CA-360, 0.5% Na-deoxycholate, 0.1% SDS) containing the protease inhibitor 1 mM PMSF. The membranes were stored at 20°C. Whole cell lysate was incubated with 2% SDS, 62.5 mM Tris, 10% glycerol, 5% β-mercaptoethanol, and 0.05% bromophenol blue for 5 minutes at 100°C. 40 μg of protein for each sample was loaded and separated on 10% polyacrylamide gels, then transferred to PVDF membranes. Blots were blocked with TBS containing 1% Tween-20 and 5% skim milk for 30 min at RT, and incubated with a goat polyclonal antibody against thrombin receptor (S-19; Santa Cruz; 1:300) overnight at 4°C. After washing with TBS plus Tween, blots were incubated with HRP-conjugated anti-goat secondary antibody (Santa Cruz; 1:3000), followed by washing and the detection of immunoreactivity with enhanced chemiluminescence (ECL; Amersham). The same blots were re-probed with a rabbit monoclonal antibody against α-actin (Sigma; catalog # A2066; 1:2000) to confirm equal loading.
The dentate gyrus was dissected from 400 μm horizontal rat brain slices, incubated with 1 mg/ml trypsin for 20 min, and then mechanically dissociated using vibration with fire polished glass pipettes. Dissociated cells are plated on glass coverslips, and loaded with 5 μM Fluo3-AM for 30 min for Ca2+ imaging. External solution contained (in mM) 150 NaCl, 10 HEPES, 3 KCl, 2 CaCl2, 1 MgCl2, 22 sucrose, 10 glucose; pH adjusted to 7.4 and osmolarity to 325 mOsm (23°C). 30 μM TFLLR or 100 μM NMDA were applied to the cells Fluo3 was excited by a 100 W mercury lamp and the timing was controlled by a high speed shutter (Uniblitz). Images were acquired and analyzed by custom software.
Whole-cell patch clamp recording of dentate granule cells
Young mice (C57/B16, age P15-20) were deeply anaesthetized with isoflurane until cessation of breathing and subsequently decapitated. The brain was rapidly removed and submerged in an ice-cold oxygenated artificial cerebrospinal fluid (ACSF) composed of (in mM) 130 NaCl, 24 NaHCO3, 3.5 KCl, 1.25 NaH2PO4, 1 CaCl2, 3 MgCl2, 10 glucose at pH 7.4, and was bubbled with 5% CO2/95% O2. Transverse slices (300 μm) were prepared with a Leica vibratome, and incubated in a chamber with oxygenated ACSF at room temperature for 1 hr before use. The internal solution was comprised of (mM) 140 K-MeSO4, 10 HEPES, 7 NaCl, 4 Mg-ATP, and 0.3 Na-GTP. The recording ACSF solution was composed of (in mM) 130 NaCl, 24 NaHCO3, 3.5 KCl, 1.25 NaH2PO4, 1.5 CaCl2, 1.5 MgCl2, and 10 glucose at pH 7.4 and was bubbled with 5% CO2/95% O2 (23°C). Visually guided whole-cell patch recordings were obtained from dentate granule neurons in current clamp configuration using an Axopatch 200A (Axon instruments, Union City, CA, USA) and a patch pipette of 5~7 MΩ resistance. Electrophysiological properties were monitored before and at the end of the experiments. Series and input resistances were monitored throughout the experiment using a -5 mV pulse. Recordings were considered stable when the series and input resistances, resting membrane potential and stimulus artifact duration did not change > 20%.
Voltage Dye Imaging
400 μm thick transverse hippocampal slices of mouse brain were loaded with the voltage dye, di-4-ANEPPS (D-1199, Molecular Probes Inc.) at 3 mg/ml for 10-30 min. The voltage sensitive dye (VSD) was dissolved into a 2:1 mixture of ethanol and 10% Cremophor EL (Sigma), a castor oil derivative, which was used as a dye stock solution (3.3 mg of VSD/ml mixture). The dye stock solution was mixed with a 1:1 mixture of ACSF and fetal bovine serum (Sigma) to a final VSD concentration of 0.2 mM and was used as staining solution. Each slice was stained with 100 ml of the staining solution by gently squirting the solution into the plexiglass ring, following incubation in a humidified chamber for 25 min. The slices were rinsed with ACSF by dipping it together with the plexiglass ring . Images (resolution: 60 × 90 pixels) were acquired at 100 Hz (10 ms sample interval) for 65 seconds (23°C), using MiCam camera system (BrainVision, Japan). This high speed camera system converted the changes in intensity to different colors. Di-4-ANEPPS decreases its fluorescence intensity when the membrane depolarizes. A 20× water objective (N.A. = 0.95, Olympus) was used to acquire the images. The dye was excited at 510 nm and emitted light that was detected at 590 nm.
400 μm transverse hippocampal slices were prepared from 21-28 day old mice, as described above. Slices (400 μm thick) were placed in a submerged chamber superfused with oxygenated ACSF (see above). Field potentials were recorded with a micropipette (5-10 MOhm) filled with HEPES-buffered saline positioned in the dentate gyrus molecular layer. Field EPSPs were evoked at room temperature (25°C) by perforant path stimulation (0.1 ms, 10-100 μA) using a monopolar stimulating electrode. The NMDA component was isolated by recording in 0.1 mM Mg2+ and 10 μM CNQX. NMDA-component field EPSPs were digitized at 10 kHz, and the field EPSP amplitude quantified.
This work is supported by NIH (NS039419 SFT; NS043875 CJL; NS042505 CEJ,) and by World Class Institute Program of Korea Ministry of Education, Science and Technology (CJL). We thank Juan Rong for sharing unpublished data.
- Landis RC: Protease activated receptors: clinical relevance to hemostasis and inflammation. Hematol Oncol Clin North Am. 2007, 21 (1): 103-113. 10.1016/j.hoc.2006.11.005.PubMedGoogle Scholar
- Tanaka KA, Key NS, Levy JH: Blood coagulation: hemostasis and thrombin regulation. Anesth Analg. 2009, 108 (5): 1433-1446. 10.1213/ane.0b013e31819bcc9c.PubMedGoogle Scholar
- Vine AK: Recent advances in haemostasis and thrombosis. Retina. 2009, 29 (1): 1-7. 10.1097/IAE.0b013e31819091dc.PubMedGoogle Scholar
- Coughlin SR: Thrombin signalling and protease-activated receptors. Nature. 2000, 407 (6801): 258-264. 10.1038/35025229.PubMedGoogle Scholar
- Coughlin SR: Protease-activated receptors in vascular biology. Thromb Haemost. 2001, 86 (1): 298-307.PubMedGoogle Scholar
- Sorensen SD, Nicole O, Peavy RD, Montoya LM, Lee CJ, Murphy TJ, Traynelis SF, Hepler JR: Common signaling pathways link activation of murine PAR-1, LPA, and S1P receptors to proliferation of astrocytes. Mol Pharmacol. 2003, 64 (5): 1199-1209. 10.1124/mol.64.5.1199.PubMedGoogle Scholar
- Traynelis SF, Trejo J: Protease-activated receptor signaling: new roles and regulatory mechanisms. Curr Opin Hematol. 2007, 14 (3): 230-235. 10.1097/MOH.0b013e3280dce568.PubMedGoogle Scholar
- Junge CE, Lee CJ, Hubbard KB, Zhang Z, Olson JJ, Hepler JR, Brat DJ, Traynelis SF: Protease-activated receptor-1 in human brain: localization and functional expression in astrocytes. Exp Neurol. 2004, 188 (1): 94-103. 10.1016/j.expneurol.2004.02.018.PubMedGoogle Scholar
- Hermann GE, Van Meter MJ, Rood JC, Rogers RC: Proteinase-activated receptors in the nucleus of the solitary tract: evidence for glial-neural interactions in autonomic control of the stomach. J Neurosci. 2009, 29 (29): 9292-9300. 10.1523/JNEUROSCI.6063-08.2009.PubMed CentralPubMedGoogle Scholar
- Wang H, Ubl JJ, Reiser G: Four subtypes of protease-activated receptors, co-expressed in rat astrocytes, evoke different physiological signaling. Glia. 2002, 37 (1): 53-63. 10.1002/glia.10012.PubMedGoogle Scholar
- Weinstein JR, Gold SJ, Cunningham DD, Gall CM: Cellular localization of thrombin receptor mRNA in rat brain: expression by mesencephalic dopaminergic neurons and codistribution with prothrombin mRNA. J Neurosci. 1995, 15 (4): 2906-2919.PubMedGoogle Scholar
- Niclou S, Suidan HS, Brown-Luedi M, Monard D: Expression of the thrombin receptor mRNA in rat brain. Cell Mol Biol (Noisy-le-grand). 1994, 40 (3): 421-428.Google Scholar
- Ide J, Aoki T, Ishivata S, Glusa E, Strukova SM: Proteinase-activated receptor agonists stimulate the increase in intracellular Ca2+ in cardiomyocytes and proliferation of cardiac fibroblasts from chick embryos. Bull Exp Biol Med. 2007, 144 (6): 760-763. 10.1007/s10517-007-0425-z.PubMedGoogle Scholar
- Di Serio C, Pellerito S, Duarte M, Massi D, Naldini A, Cirino G, Prudovsky I, Santucci M, Geppetti P, Marchionni N, Masotti G, Tarantini F: Protease-activated receptor 1-selective antagonist SCH79797 inhibits cell proliferation and induces apoptosis by a protease-activated receptor 1-independent mechanism. Basic Clin Pharmacol Toxicol. 2007, 101 (1): 63-69. 10.1111/j.1742-7843.2007.00078.x.PubMedGoogle Scholar
- Wang H, Ubl JJ, Stricker R, Reiser G: Thrombin (PAR-1)-induced proliferation in astrocytes via MAPK involves multiple signaling pathways. Am J Physiol Cell Physiol. 2002, 283 (5): C1351-1364.PubMedGoogle Scholar
- Nicole O, Goldshmidt A, Hamill CE, Sorensen SD, Sastre A, Lyuboslavsky P, Hepler JR, McKeon RJ, Traynelis SF: Activation of protease-activated receptor-1 triggers astrogliosis after brain injury. J Neurosci. 2005, 25 (17): 4319-4329. 10.1523/JNEUROSCI.5200-04.2005.PubMedGoogle Scholar
- Lee CJ, Mannaioni G, Yuan H, Woo DH, Gingrich MB, Traynelis SF: Astrocytic control of synaptic NMDA receptors. J Physiol. 2007, 581 (Pt 3): 1057-1081.PubMed CentralPubMedGoogle Scholar
- Cannon JR, Keep RF, Schallert T, Hua Y, Richardson RJ, Xi G: Protease-activated receptor-1 mediates protection elicited by thrombin preconditioning in a rat 6-hydroxydopamine model of Parkinson's disease. Brain Res. 2006, 1116 (1): 177-186. 10.1016/j.brainres.2006.07.094.PubMedGoogle Scholar
- Cannon JR, Hua Y, Richardson RJ, Xi G, Keep RF, Schallert T: The effect of thrombin on a 6-hydroxydopamine model of Parkinson's disease depends on timing. Behav Brain Res. 2007, 183 (2): 161-168. 10.1016/j.bbr.2007.06.004.PubMed CentralPubMedGoogle Scholar
- Nagai T, Nabeshima T, Yamada K: Basic and translational research on proteinase-activated receptors: regulation of nicotine reward by the tissue plasminogen activator (tPA) - plasmin system via proteinase-activated receptor 1. J Pharmacol Sci. 2008, 108 (4): 408-414. 10.1254/jphs.08R04FM.PubMedGoogle Scholar
- Striggow F, Riek-Burchardt M, Kiesel A, Schmidt W, Henrich-Noack P, Breder J, Krug M, Reymann KG, Reiser G: Four different types of protease-activated receptors are widely expressed in the brain and are up-regulated in hippocampus by severe ischemia. Eur J Neurosci. 2001, 14 (4): 595-608. 10.1046/j.0953-816x.2001.01676.x.PubMedGoogle Scholar
- Laskowski A, Reiser G, Reymann KG: Protease-activated receptor-1 induces generation of new microglia in the dentate gyrus of traumatised hippocampal slice cultures. Neurosci Lett. 2007, 415 (1): 17-21. 10.1016/j.neulet.2006.12.050.PubMedGoogle Scholar
- Qiao L, Zhang H, Wu S, He S: Downregulation of protease activated receptor expression and cytokine production in P815 cells by RNA interference. BMC Cell Biol. 2009, 10: 62-10.1186/1471-2121-10-62.PubMed CentralPubMedGoogle Scholar
- Smith-Swintosky VL, Zimmer S, Fenton JW, Mattson MP: Protease nexin-1 and thrombin modulate neuronal Ca2+ homeostasis and sensitivity to glucose deprivation-induced injury. J Neurosci. 1995, 15 (8): 5840-5850.PubMedGoogle Scholar
- Yang Y, Akiyama H, Fenton JW, Brewer GJ: Thrombin receptor on rat primary hippocampal neurons: coupled calcium and cAMP responses. Brain Res. 1997, 761 (1): 11-18. 10.1016/S0006-8993(97)00311-9.PubMedGoogle Scholar
- Smirnova IV, Vamos S, Wiegmann T, Citron BA, Arnold PM, Festoff BW: Calcium mobilization and protease-activated receptor cleavage after thrombin stimulation in motor neurons. J Mol Neurosci. 1998, 10 (1): 31-44. 10.1007/BF02737083.PubMedGoogle Scholar
- Suo Z, Wu M, Ameenuddin S, Anderson HE, Zoloty JE, Citron BA, Andrade-Gordon P, Festoff BW: Participation of protease-activated receptor-1 in thrombin-induced microglial activation. J Neurochem. 2002, 80 (4): 655-666. 10.1046/j.0022-3042.2001.00745.x.PubMedGoogle Scholar
- Gingrich MB, Junge CE, Lyuboslavsky P, Traynelis SF: Potentiation of NMDA receptor function by the serine protease thrombin. J Neurosci. 2000, 20 (12): 4582-4595.PubMedGoogle Scholar
- Lee KH, Cho JH, Choi IS, Park HM, Lee MG, Choi BJ, Jang IS: Pregnenolone sulfate enhances spontaneous glutamate release by inducing presynaptic Ca2+-induced Ca2+ release. Neuroscience. 2010, 171 (1): 106-116. 10.1016/j.neuroscience.2010.07.057.PubMedGoogle Scholar
- Li Z, Hatton GI: Histamine-induced prolonged depolarization in rat supraoptic neurons: G-protein-mediated, Ca(2+)-independent suppression of K+ leakage conductance. Neuroscience. 1996, 70 (1): 145-158. 10.1016/0306-4522(95)00373-Q.PubMedGoogle Scholar
- Smith BN, Armstrong WE: The ionic dependence of the histamine-induced depolarization of vasopressin neurones in the rat supraoptic nucleus. J Physiol. 1996, 495 (Pt 2): 465-478.PubMed CentralPubMedGoogle Scholar
- Zhou J, Lee AW, Devidze N, Zhang Q, Kow LM, Pfaff DW: Histamine-induced excitatory responses in mouse ventromedial hypothalamic neurons: ionic mechanisms and estrogenic regulation. J Neurophysiol. 2007, 98 (6): 3143-3152. 10.1152/jn.00337.2007.PubMedGoogle Scholar
- Mannaioni G, Marino MJ, Valenti O, Traynelis SF, Conn PJ: Metabotropic glutamate receptors 1 and 5 differentially regulate CA1 pyramidal cell function. J Neurosci. 2001, 21 (16): 5925-5934.PubMedGoogle Scholar
- Mannaioni G, Orr AG, Hamill CE, Yuan H, Pedone KH, McCoy KL, Berlinguer Palmini R, Junge CE, Lee CJ, Yepes M, Hepler JR, Traynelis SF: Plasmin potentiates synaptic N-methyl-D-aspartate receptor function in hippocampal neurons through activation of protease-activated receptor-1. J Biol Chem. 2008, 283 (29): 20600-20611. 10.1074/jbc.M803015200.PubMed CentralPubMedGoogle Scholar
- Oliet SH, Mothet JP: Regulation of N-methyl-D-aspartate receptors by astrocytic D-serine. Neuroscience. 2009, 158 (1): 275-283. 10.1016/j.neuroscience.2008.01.071.PubMedGoogle Scholar
- Eichholtz T, Jalink K, Fahrenfort I, Moolenaar WH: The bioactive phospholipid lysophosphatidic acid is released from activated platelets. Biochem J. 1993, 291 (Pt 3): 677-680.PubMed CentralPubMedGoogle Scholar
- Miller B, Sarantis M, Traynelis SF, Attwell D: Potentiation of NMDA receptor currents by arachidonic acid. Nature. 1992, 355 (6362): 722-725. 10.1038/355722a0.PubMedGoogle Scholar
- Holtsberg FW, Steiner MR, Furukawa K, Keller JN, Mattson MP, Steiner SM: Lysophosphatidic acid induces a sustained elevation of neuronal intracellular calcium. J Neurochem. 1997, 69 (1): 68-75.PubMedGoogle Scholar
- Baranes D, Lederfein D, Huang YY, Chen M, Bailey CH, Kandel ER: Tissue plasminogen activator contributes to the late phase of LTP and to synaptic growth in the hippocampal mossy fiber pathway. Neuron. 1998, 21 (4): 813-825. 10.1016/S0896-6273(00)80597-8.PubMedGoogle Scholar
- Nagai T, Ito M, Nakamichi N, Mizoguchi H, Kamei H, Fukakusa A, Nabeshima T, Takuma K, Yamada K: The rewards of nicotine: regulation by tissue plasminogen activator-plasmin system through protease activated receptor-1. J Neurosci. 2006, 26 (47): 12374-12383. 10.1523/JNEUROSCI.3139-06.2006.PubMedGoogle Scholar
- Almonte AG, Hamill CE, Chhatwal JP, Wingo TS, Barber JA, Lyuboslavsky PN, David Sweatt J, Ressler KJ, White DA, Traynelis SF: Learning and memory deficits in mice lacking protease activated receptor-1. Neurobiol Learn Mem. 2007, 88 (3): 295-304. 10.1016/j.nlm.2007.04.004.PubMed CentralPubMedGoogle Scholar
- Tomimatsu Y, Idemoto S, Moriguchi S, Watanabe S, Nakanishi H: Proteases involved in long-term potentiation. Life Sci. 2002, 72 (4-5): 355-361. 10.1016/S0024-3205(02)02285-3.PubMedGoogle Scholar
- Maggio N, Shavit E, Chapman J, Segal M: Thrombin induces long-term potentiation of reactivity to afferent stimulation and facilitates epileptic seizures in rat hippocampal slices: toward understanding the functional consequences of cerebrovascular insults. J Neurosci. 2008, 28 (3): 732-736. 10.1523/JNEUROSCI.3665-07.2008.PubMedGoogle Scholar
- Junge CE, Sugawara T, Mannaioni G, Alagarsamy S, Conn PJ, Brat DJ, Chan PH, Traynelis SF: The contribution of protease-activated receptor 1 to neuronal damage caused by transient focal cerebral ischemia. Proc Natl Acad Sci USA. 2003, 100 (22): 13019-13024. 10.1073/pnas.2235594100.PubMed CentralPubMedGoogle Scholar
- Hamill CE, Mannaioni G, Lyuboslavsky P, Sastre AA, Traynelis SF: Protease-activated receptor 1-dependent neuronal damage involves NMDA receptor function. Exp Neurol. 2009, 217 (1): 136-146. 10.1016/j.expneurol.2009.01.023.PubMed CentralPubMedGoogle Scholar
- Pinet C, Algalarrondo V, Sablayrolles S, Le Grand B, Pignier C, Cussac D, Perez M, Hatem SN, Coulombe A: Protease-activated receptor-1 mediates thrombin-induced persistent sodium current in human cardiomyocytes. Mol Pharmacol. 2008, 73 (6): 1622-1631. 10.1124/mol.107.043182.PubMedGoogle Scholar
- Strande JL, Hsu A, Su J, Fu X, Gross GJ, Baker JE: SCH 79797, a selective PAR1 antagonist, limits myocardial ischemia/reperfusion injury in rat hearts. Basic Res Cardiol. 2007, 102 (4): 350-358. 10.1007/s00395-007-0653-4.PubMed CentralPubMedGoogle Scholar
- Tsuboi H, Naito Y, Katada K, Takagi T, Handa O, Kokura S, Ichikawa H, Yoshida N, Tsukada M, Yoshikawa T: Role of the thrombin/protease-activated receptor 1 pathway in intestinal ischemia-reperfusion injury in rats. Am J Physiol Gastrointest Liver Physiol. 2007, 292 (2): G678-683.PubMedGoogle Scholar
- Henrich-Noack P, Riek-Burchardt M, Baldauf K, Reiser G, Reymann KG: Focal ischemia induces expression of protease-activated receptor1 (PAR1) and PAR3 on microglia and enhances PAR4 labeling in the penumbra. Brain Res. 2006, 1070 (1): 232-241. 10.1016/j.brainres.2005.10.100.PubMedGoogle Scholar
- Olson EE, Lyuboslavsky P, Traynelis SF, McKeon RJ: PAR-1 deficiency protects against neuronal damage and neurologic deficits after unilateral cerebral hypoxia/ischemia. J Cereb Blood Flow Metab. 2004, 24 (9): 964-971.PubMedGoogle Scholar
- Chintala M, Shimizu K, Ogawa M, Yamaguchi H, Doi M, Jensen P: Basic and translational research on proteinase-activated receptors: antagonism of the proteinase-activated receptor 1 for thrombin, a novel approach to antiplatelet therapy for atherothrombotic disease. J Pharmacol Sci. 2008, 108 (4): 433-438. 10.1254/jphs.08R06FM.PubMedGoogle Scholar
- Sharp F, Liu DZ, Zhan X, Ander BP: Intracerebral hemorrhage injury mechanisms: glutamate neurotoxicity, thrombin, and Src. Acta Neurochir Suppl. 2008, 105: 43-46. 10.1007/978-3-211-09469-3_9.PubMedGoogle Scholar
- Fujimoto S, Katsuki H, Kume T, Akaike A: Thrombin-induced delayed injury involves multiple and distinct signaling pathways in the cerebral cortex and the striatum in organotypic slice cultures. Neurobiol Dis. 2006, 22 (1): 130-142. 10.1016/j.nbd.2005.10.008.PubMedGoogle Scholar
- Choi SH, Lee DY, Ryu JK, Kim J, Joe EH, Jin BK: Thrombin induces nigral dopaminergic neurodegeneration in vivo by altering expression of death-related proteins. Neurobiol Dis. 2003, 14 (2): 181-193. 10.1016/S0969-9961(03)00085-8.PubMedGoogle Scholar
- Hamill CE, Goldshmidt A, Nicole O, McKeon RJ, Brat DJ, Traynelis SF: Special lecture: glial reactivity after damage: implications for scar formation and neuronal recovery. Clin Neurosurg. 2005, 52: 29-44.PubMedGoogle Scholar
- Lee KR, Drury I, Vitarbo E, Hoff JT: Seizures induced by intracerebral injection of thrombin: a model of intracerebral hemorrhage. J Neurosurg. 1997, 87 (1): 73-78. 10.3171/jns.1997.87.1.0073.PubMedGoogle Scholar
- Tominaga T, Tominaga Y, Yamada H, Matsumoto G, Ichikawa M: Quantification of optical signals with electrophysiological signals in neural activities of Di-4-ANEPPS stained rat hippocampal slices. J Neurosci Methods. 2000, 102 (1): 11-23. 10.1016/S0165-0270(00)00270-3.PubMedGoogle Scholar
This article is published under license to BioMed Central Ltd. This is an Open Access article distributed under the terms of the Creative Commons Attribution License (http://creativecommons.org/licenses/by/2.0), which permits unrestricted use, distribution, and reproduction in any medium, provided the original work is properly cited.