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Selective Activation of KCa3.1 and CRAC Channels by P2Y2 Receptors Promotes Ca2+ Signaling, Store Refilling and Migration of Rat Microglial Cells

  • Roger Ferreira,

    Affiliations Genes and Development Division, Toronto Western Research Institute, University Health Network, Toronto, Ontario, Canada, Department of Physiology, University of Toronto, Toronto, Ontario, Canada

  • Lyanne C. Schlichter

    schlicht@uhnres.utoronto.ca

    Affiliations Genes and Development Division, Toronto Western Research Institute, University Health Network, Toronto, Ontario, Canada, Department of Physiology, University of Toronto, Toronto, Ontario, Canada

Selective Activation of KCa3.1 and CRAC Channels by P2Y2 Receptors Promotes Ca2+ Signaling, Store Refilling and Migration of Rat Microglial Cells

  • Roger Ferreira, 
  • Lyanne C. Schlichter
PLOS
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Abstract

Microglial activation involves Ca2+ signaling, and numerous receptors can evoke elevation of intracellular Ca2+. ATP released from damaged brain cells can activate ionotropic and metabotropic purinergic receptors, and act as a chemoattractant for microglia. Metabotropic P2Y receptors evoke a Ca2+ rise through release from intracellular Ca2+ stores and store-operated Ca2+ entry, and some have been implicated in microglial migration. This Ca2+ rise is expected to activate small-conductance Ca2+-dependent K+ (SK) channels, if present. We previously found that SK3 (KCa2.3) and KCa3.1 (SK4/IK1) are expressed in rat microglia and contribute to LPS-mediated activation and neurotoxicity. However, neither current has been studied by elevating Ca2+ during whole-cell recordings. We hypothesized that, rather than responding only to Ca2+, each channel type might be coupled to different receptor-mediated pathways. Here, our objective was to determine whether the channels are differentially activated by P2Y receptors, and, if so, whether they play differing roles. We used primary rat microglia and a rat microglial cell line (MLS-9) in which riluzole robustly activates both SK3 and KCa3.1 currents. Using electrophysiological, Ca2+ imaging and pharmacological approaches, we show selective functional coupling of KCa3.1 to UTP-mediated P2Y2 receptor activation. KCa3.1 current is activated by Ca2+ entry through Ca2+-release-activated Ca2+ (CRAC/Orai1) channels, and both CRAC/Orai1 and KCa3.1 channels facilitate refilling of Ca2+ stores. The Ca2+ dependence of KCa3.1 channel activation was skewed to abnormally high concentrations, and we present evidence for a close physical association of the two channel types. Finally, migration of primary rat microglia was stimulated by UTP and inhibited by blocking either KCa3.1 or CRAC/Orai1 channels. This is the first report of selective coupling of one type of SK channel to purinergic stimulation of microglia, transactivation of KCa3.1 channels by CRAC/Orai1, and coordinated roles for both channels in store refilling, Ca2+ signaling and microglial migration.

Introduction

In the mature CNS, microglial cells with highly branched processes continually survey the local microenvironment and rapidly respond to stranger and danger signals [1]. Migration to the site of damage is an essential component of the microglial response to acute CNS injury. ATP, which is released from damaged cells, can bind to microglial ionotropic (P2X) and metabotropic (P2Y) purinergic receptors and promote migration [2][4]. In vitro studies on microglia migration have focused on the roles of P2X4 and P2Y12 [5][7]. Microglial P2Y receptors rapidly elevate intracellular free Ca2+ by coupling Ca2+ release from stores to store operated Ca2+ entry (SOCE) [8], [9]. Thus, it is expected that P2Y receptors will link extracellular damage signals to intracellular Ca2+, microglial activation and migration. The SOCE pathway used by microglia for migration following P2Y receptor activation has not been identified. By combining molecular, biophysical and pharmacological approaches, we previously identified the Ca2+-release activated Ca2+ (CRAC) channel as a major SOCE pathway in primary rat microglia [10]. More recently, we discovered a contribution of CRAC channels to microglial migration and the formation of podosomes [11].

An expected immediate response to elevated intracellular Ca2+ in microglia is opening of SK (small-conductance Ca2+-activated K+) channels. We previously showed that SK4 (KCa3.1) [12] and SK3 (KCa2.3) channels [13] are expressed in rat microglia, and regulate activation evoked by lipopolysaccharide; i.e., p38MAPK activation, iNOS up-regulation and nitric oxide production, and the ability of microglia to kill neurons. At the time, we hypothesized that the SK channels contribute to microglial activation by maintaining a negative membrane potential and thus, a large driving force for Ca2+ influx through CRAC channels. However, the SK currents were not monitored, and roles of SK3 and KCa3.1 channels in regulating SOCE have not been examined in microglia. Recently, we discovered that both SK3 and KCa3.1 currents are reliably activated in the MLS-9 microglia cell line by the neuroprotective drug, riluzole, with little or no rise in intracellular Ca2+ [14]. This finding contradicts the prevailing view that riluzole simply sensitizes SK channels so that they open at resting Ca2+ levels [15]. Furthermore, neither SK3 nor KCa3.1 current was activated simply by raising Ca2+ to ∼1 µM, which is well above the normal EC50 values reported for native and heterologously expressed channels (see Discussion). Instead, our results on MLS-9 cells raise the possibility that SK3 and KCa3.1 channels in microglia require more than a simple elevation in Ca2+. If so, it is possible that the two channel types can selectively respond to different stimuli.

This study was designed to address three overall questions. First, we asked whether metabotropic P2Y2 receptors in microglia elevate intracellular Ca2+ and activate SK3 and KCa3.1 channels, and if so, whether this requires Ca2+ entry through CRAC channels. Having found that only KCa3.1 channels were activated, and that CRAC channels were involved, we next asked whether KCa3.1 channels selectively control store-operated Ca2+ entry and store refilling. This was the case. Finally, we asked whether P2Y2 receptors increase microglia migration through mechanisms that require CRAC and the selective activation of KCa3.1. Again, we found this to be the case.

Materials and Methods

Cells

Ethics statement.

Animals were used in strict accordance with the guidelines established by the Canadian Council on Animal Care, and was approved by the Animal Care Committee of the University Health Network (AUP #914). Primary cultures of rat microglia (≥98% pure) were prepared from brains harvested from 1–2 day old Sprague Dawley pups (Charles River, St-Constant, Quebec, Canada) Essentially pure microglia cultures were prepared according to our standard protocols [10], [12], [13], [16]. That is, following removal of the meninges, the brain was minced in cold Minimal Essential Medium (MEM; Invitrogen, Burlington, ON, Canada). The dissociated tissue was centrifuged (300×g, 10 min) and re-suspended in MEM supplemented with 10% fetal bovine serum (FBS) (from Wisent, St-Bruno, PQ), and 0.05 mg/mL gentamycin (Invitrogen). After two days growth in tissue culture flasks, the supernatant containing cellular debris and non-adherent cells was removed and replaced with fresh medium. The mixed cell cultures were allowed to grow for another 8 days, and were then shaken on an orbital shaker (65 rpm, 3–4 h, 37°C, 5% CO2). The resulting suspension of non-adherent microglia was centrifuged (300×g, 10 min), the pellet was re-suspended in MEM with reduced serum (2% FBS). Under these conditions, we have found that the microglial cells are a relatively non-activated state [16].

Our laboratory derived the MLS-9 cell line many years ago by treating pure cultures of rat microglia with colony stimulating factor-1 for several weeks. Individual cell colonies were harvested and used to establish continuous cell lines, of which we named one, MLS-9 [17]. We have used this cell line extensively for studies of K+ channels [14], [17][20] and Cl channels [21]. MLS-9 cells were thawed and cultured for several days in culture medium (MEM, 10% FBS, 100 µM gentamycin), and then harvested in phosphate buffered saline (PBS) containing 0.25% trypsin and 1 mM EDTA, washed with MEM, centrifuged (300×g, 10 min) and re-suspended in culture medium. MLS-9 cells were plated in the culture medium at 4.5×104 cells/coverslip for Ca2+ imaging and patch-clamp analysis. An important advantage of using MLS-9 cells is that they lack three currents that can interfere with isolating Ca2+-activated K+ currents. Primary rat microglia have an inward-rectifier K+ current at negative membrane potentials [22], [23], a large outward Kv1.3 current that activates above about −30 mV [22], and TRPM7, which produces a large current at positive potentials [24].

Chemicals were from Sigma-Aldrich, unless otherwise indicated. Stock solutions of several antagonists were made with DMSO; i.e., the P2Y receptor blocker, suramin, the Orai1/CRAC blockers 2-APB and BTP2, and the KCa3.1 blocker, TRAM-34. Uridine 5′-triphosphate (trisodium salt dehydrate) and the SK1-SK3 blocker, apamin, were dissolved in double distilled water. All stock solutions were aliquoted and stored at –20°C until used.

Intracellular free Ca2+

The Fura-2 imaging methods were the same as we recently described [14]. MLS-9 cells growing on glass coverslips (∼5×104 cells per 15 mm diameter coverslip) were incubated at room temperature with 3.5 µg/ml Fura-2AM (Invitrogen) for 45 min in the dark. A coverslip was then mounted in a 300 µl volume perfusion chamber (Model RC-25, Warner Instruments, Hamden CT), containing the same bath solution as for patch-clamping (see below). The effects of ion channel blockers (50 µM 2-APB, 10 µM BTP2, 1 µM TRAM-34, 100 nM apamin) on UTP-evoked calcium signals were assessed on different batches of cells from separate coverslips. Images were acquired at room temperature using a Nikon Diaphot inverted microscope, Retiga-EX camera (Q-Imaging, Burnaby, BC, Canada), and Northern Eclipse image acquisition software (Empix Imaging, Mississauga, ON, Canada). A Lambda DG-4 Ultra High Speed Wavelength Switcher (Sutter Instruments, Novato, CA) was used to alternately acquire images at 340 and 380 nm excitation wavelengths. Images were acquired every 4 s, and the excitation shutter was closed between acquisitions to prevent photobleaching. The intracellular free Ca2+ concentration was calculated from the standard equation [25] as before [14]. For every experiment, cells on a matched coverslip (i.e., not exposed to UTP) were exposed to 2 µM ionomycin to obtain the maximum 340∶380 ratio with saturating calcium. Then, a Ca2+-free bath solution with 2 µM ionomycin and 3 mM MnCl2 was perfused in to obtain the minimum 340∶380 ratio.

Patch-clamp electrophysiology

MLS-9 cells were plated on 15 mm diameter coverslips (4.5×104/coverslip), mounted in the same perfusion chamber as for Ca2+ imaging. The cells were superfused with an extracellular (bath) solution containing the following (in mM): 125 NaCl, 5 KCl, 1 MgCl2, 1 CaCl2, 5 glucose, and 10 HEPES, adjusted to pH 7.4 (with NaOH) and to ∼300 mOsm with sucrose. For Ca2+-free bath solution, CaCl2 was omitted and 1 mM EGTA was added. Bath solutions were exchanged using a gravity-driven perfusion system flowing at 1.5–2 ml/min and all recordings were made at room temperature. Whole-cell recordings were made with pipettes pulled from thin-walled borosilicate glass (WPI, Sarasota, FL) to a resistance of 5–8 MΩ using a Narishige puller (Narishige Scientific, Setagaya-Ku, Tokyo). Pipettes were filled with a solution (intracellular) containing (in mM): 100 K-aspartate, 40 KCl, 1 MgCl2, 2 MgATP, and 10 HEPES, pH adjusted to 7.2 (with KOH), 280 mOsm/kgH2O. Either 1 EGTA+0.5 CaCl2 or 1 BAPTA+0.45 CaCl2 (where noted) was used to buffer the initial internal free Ca2+ to ∼120 nM (calculated using WEBMAXC Extended software, http://www.stanford.edu/~cpatton/webmaxc/webmaxcE.htm). We chose low buffer concentrations (1 mM) to allow the purinergic receptor agonist, UTP, to transiently elevate intracellular Ca2+. Recordings were made with an Axon Multiclamp 700A amplifier, compensated on-line for capacitance and series resistance. Patch-clamp data were filtered at 5 kHz, and acquired and digitized using a Digidata 1322A board with pClamp software. Junction potentials were reduced by using agar bridges made with bath solution, and were calculated with the utility in pCLAMP. After correction, all reported voltages were about 5 mV more negative than reported in the text and figures.

Immunocytochemistry

Standard methods were used, similar to our recent papers [11], [13], [26]. In brief, antibodies were diluted in 4% donkey serum and centrifuged (8200×g, 10 min) to precipitate any aggregated antibody. MLS-9 cells were fixed for 10 min in 4% paraformaldehyde and washed (3×, 5 min each). This was followed by antigen retrieval in hot citrate buffer, which we found necessary for optimal Orai1 staining [11]. Cells were washed and permeabilized for 5 min with 0.2% Triton X-100, and washed in PBS (3×, 5 min each). Non-specific antigens were blocked with 4% donkey serum for 1 h at room temperature. The cells were then incubated with the following primary antibodies overnight at 4°C: anti-Orai1 (goat polyclonal, 1∶100; Santa Cruz Biotechnology; Santa Cruz, CA), and anti-KCa3.1 (SK4) (rabbit polyclonal, anti-serum, 1∶1000; Abcam; Cambridge, MA). The cells were washed in PBS (4×, 5 min each), followed by another block with 4% donkey serum and 0.01% BSA for 1 h at room temperature. The cells were then incubated (1 h, room temperature) with the secondary antibodies: Alexa Fluor 488-conjugated (green) bovine anti-goat (1∶1000; Jackson Immunoresearch; West Grove, PA, USA), and DyLight 594-conjugated (red) donkey anti-rabbit (1∶250; Jackson Immunoresearch; West Grove, PA, USA). Negative controls were prepared using the same protocol, but omitting each primary antibody. After washing in PBS (4×, 5 min each) cell nuclei were labelled for 5 min with DAPI (4′-6-diamidino-2-phenylindole) (1∶3000; Sigma-Aldrich), and then washed in PBS (3×, 5 min each). The coverslips were mounted on glass slides with DAKO mounting medium (Dako; Glostrup, Denmark). Cells were imaged with an Axioplan 2 microscope using a 63× objective lens. Images were recorded with an Axiocam HRm digital camera, deconvolved and analyzed with Axiovision 4.6 software (all from Zeiss; Toronto, ON).

TranswellTM migration assay

Cultured primary rat microglia (2–3×104 cells/insert) were seeded on the upper inserts of 24-well TranswellTM Migration Chambers (VWR, Mississauga, ON), which contained uncoated filters with open 8 µm-diameter holes. Microglia were bathed in MEM with 2% FBS and allowed to adhere for ∼1 h prior to adding compounds. When used, UTP was added to the lower well to act as a chemoattractant, and each antagonist was added to the upper well. The chamber was incubated (24 h, 37°C, 5% CO2). To quantify the transmigration of microglia to the underside of each filter, we first removed the remaining cells from the upper side, using a Q-tipTM. The filters were fixed (4% PFA, 15 min), rinsed 3× in PBS, stained with 0.5% crystal violet (1 min), quickly rinsed, and allowed to air dry. Microglia that had migrated to the underside of each filter were viewed at 20× with an Olympus CK2 Phase Contrast Inverted microscope (Olympus, Tokyo, Japan). Cells were counted in 5 fields of view per filter.

Statistical analysis

All data are expressed as mean ± SEM. For analysis of drug effects on currents, Ca2+ signaling, and microglia migration, 1-way ANOVA and Tukey's post-hoc tests for multiple comparisons were conducted using GraphPad Prism ver 5.01 (GraphPad Software, San Diego, CA). Values of p<0.05 were taken as statistically significant.

Results

UTP activates a KCa3.1 current: Requirement for high intracellular Ca2+

The metabotropic purinergic receptor agonist, UTP, induced a biphasic Ca2+ rise, with an initial rapid increase and a more slowly decaying phase (Fig. 1A). The Ca2+ concentration was calculated by determining the maximal and minimal 340/380 values (example shown in inset, and see Methods) for each cell. For this cell, Ca2+ rapidly increased to ∼4 µM, spontaneously declined, and then returned to baseline after UTP was washed out (Fig. 1B). On average, the peak Ca2+ level was 5.3±1.2 µM (n = 19). After UTP was washed out, Ca2+ decreased to ∼85 nM, which is similar to our previous results for MLS-9 cells [14].

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Figure 1. The metabotropic purinergic receptor agonist, UTP, elevates Ca2+ elevation and selectively activates a KCa3.1 current.

A. A representative Fura-2 recording from an MLS-9 cell (rat microglia cell line), in which 100 µM UTP was bath applied during the period marked by the horizontal bar. The inset shows how the Ca2+ signal was calibrated by adding ionomycin and MnCl2, and as described in the Methods. B. The time course of the calibrated UTP-evoked Ca2+ rise (in µM) is shown for the cell in panel A. C. In whole-cell patch-clamp recordings, UTP evoked a large, transient current. From a holding potential of −70 mV, a voltage step to +50 mV was followed by a ramp from −100 to +80 mV applied every 5 sec. The two traces show the baseline control current (standard bath solution) and at the peak after adding 100 µM UTP. The reversal potential is indicated by the arrow. D. The time course of the current measured at +80 mV (same cell as panel C) is plotted on the same time scale as the Ca2+ signal in panel B. Vertical dashed lines indicate the time at which UTP was added. E. Comparison of the mean time to peak response after adding UTP for the Ca2+ signal and current activation. F. Comparison of the time course (half time) of the decay phase of the Ca2+ signal and current. G. UTP selectively activates a KCa3.1 current. The UTP-dependent current was quantified after subtracting the baseline from the maximal current (both at +80 mV) in the absence (control) or presence of the P2Y2 and P2Y6 receptor antagonist, 100 µM suramin. UTP-evoked currents were recorded in separate cells with the selective KCa3.1 blocker (1 µM TRAM-34) or the SK1–SK3 blocker (100 nM apamin) in the bath. The number of cells is indicated on each bar. ***p<0.001

https://doi.org/10.1371/journal.pone.0062345.g001

The MLS-9 microglia cell line has several of the same ion channels as primary rat microglia, and we have extensively used these cells. MLS-9 cells have important advantages for studying small-conductance Ca2+-activated K+ channels. Both SK3 (KCa2.3) and KCa3.1 currents are reliably activated (by riluzole) [14], and we have not detected voltage-gated or TRPM7 currents, which complicate the recordings from primary rat microglia. In the present study, the first surprising finding was that UTP selectively activated a large KCa3.1 current, which was identified as follows. UTP activated a current in all cells tested (n>30). The outward current showed no time dependence during voltage-clamp steps (Fig. 1C), and thus current was seen at all voltages tested with the ramp protocol (−100 to +80 mV). The reversal potential was about −75 mV (−80 mV after junction potential correction), which is very close to the K+ Nernst potential (−85 mV) with the bath and pipette solutions used. The UTP-evoked K+ current was transient (Fig. 1D), and its peak was delayed (32±5 s; n = 6) compared with the rapid Ca2+ rise (16±1 s, n = 23) (Fig. 1E). Instead, the decay phase of the current temporally matched the decay of the Ca2+ signal. The half-time (t½) for the Ca2+ decay was 56±2 s (n = 21) and 68±12 s (n = 4) for the current (Fig. 1F). This temporal relationship suggests that, rather than the initial Ca2+ rise, it is the secondary phase of the Ca2+ signal that is responsible for activating KCa3.1. The pharmacological data (Fig. 1G) show that the amplitude (358±41 pA at +80 mV; n = 6) was reduced to 116±30 pA (n = 4) by the P2Y2/P2Y6 receptor antagonist, suramin [27], and to 60.2±14.1 pA by the KCa3.1-selective blocker, TRAM-34 (n = 6). The SK1–SK3 blocker, apamin, had no effect. Thus, we conclude that UTP selectively activated KCa3.1 current. The pharmacology—activation by 100 µM UTP, inhibition by 100 µM suramin—implicates the P2Y2 receptor (see Discussion) in trans-activating KCa3.1.

The peak of the UTP-response reached a high Ca2+ level (5.3 µM); therefore, we next examined the Ca2+-dependence of current activation without UTP. Whole-cell recordings were established with pipette solutions containing 2.5, 5.2, 8.0, 10.9 or 15.3 µM free Ca2+. The bath contained apamin to preclude any possible contribution of SK3. The example cell shows activation of KCa3.1 current with 10.9 µM intracellular Ca2+ (Fig. 2A), a gradual increase to a peak at ∼3 min and a quasi-stable plateau (Fig. 2B). The current was KCa3.1, as shown by the rapid block by TRAM-34 in a separate cell (Fig. 2C). A Ca2+ dose-response curve was constructed by plotting current density (pA/pF) versus intracellular free Ca2+ (Fig. 2D). It includes our previous data with 1.1 µM (n = 10 [14]) and 0.1 µM Ca2+ (n>100 [14], and unpublished). From this relationship, the maximal current density was 23.6±2.9 pA/pF, the EC50 was 7.6±0.7 µM, and the Hill coefficient was 4.6±1.7. Similar EC50 and Hill coefficient values were obtained using current density or slope conductance. Surprisingly, this EC50 is well above the previously reported sub-micromolar values for heterologously expressed KCa3.1 channels (see Discussion), and there was no current at 1.1 µM Ca2+.

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Figure 2. KCa3.1 current activation requires unexpectedly high intracellular free Ca2+.

For these experiments on MLS-9 cells, the bath contained 100 nM apamin to eliminate any possible contribution of SK3. A. The two traces (same voltage protocol as in Fig 1) show a small current immediately after establishing the whole-cell recording (0 min) and 3 min later. The pipette solution contained 10.9 µM free Ca2+. B, C. The time course of the current measured at +80 mV is shown for two cells with 10.9 µM free intracellular Ca2+. The cell in panel A is shown in B. For a different cell (panel C), the KCa3.1 blocker, 1 µM TRAM-34, was added to the bath after the current reached a plateau, and then washed out with standard bath solution. D. Ca2+-dependence of KCa3.1 current activation. The current density (pA/pF) as a function of intracellular free Ca2+ is fitted to the Hill equation. The maximal current density is indicated by the dashed line, and the EC50 is indicated by the vertical arrow.

https://doi.org/10.1371/journal.pone.0062345.g002

KCa3.1 requires store-operated Ca2+ entry and promotes store refilling

In microglia, as in other cell types, activation of metabotropic purinergic receptors causes IP3-mediated release of Ca2+ from intracellular stores, followed by store-operated Ca2+ entry and store refilling [8]. In the MLS-9 microglia cell line, UTP evoked a P2Y receptor-mediated biphasic rise in Ca2+ (Fig. 1A,B) and activated a KCa3.1 current (Figs. 1C–E, Fig. 2). To assess whether the transient KCa3.1 activation requires Ca2+ influx, we compared the UTP-evoked current with and without Ca2+ in the bath (Fig. 3A). The summarized data (Fig. 3D) show that removing external Ca2+ decreased the current amplitude by 71%, from 358±41 pA (n = 6, same cells as in Fig. 1E) to 104±23 pA (n = 4). This demonstrates a need for Ca2+ influx. We previously showed that store-operated Ca2+ entry into rat microglia involves currents mediated by the Ca2+-release activated Ca2+ (CRAC) channel [10], whose pore-forming subunit is Orai1 [28]. To analyze whether Ca2+ influx through CRAC channels is needed to activate KCa3.1 current, we used 50 µM 2-APB (Fig. 3B, D), a concentration that blocks CRAC/Orai1 channels [29], and the more selective CRAC/Orai1 blocker, 10 µM BTP2 [30], [31] (Fig. 3C, D). The KCa3.1 current was greatly reduced by both blockers; i.e., by 72% with 2-APB (to 102±34 pA, n = 4) and by 75% with BTP2 (to 90±11 pA, n = 4). Together, these results implicate Ca2+ influx through CRAC channels in activating KCa3.1 channels after P2Y receptor stimulation.

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Figure 3. The UTP-evoked KCa3.1 current activation involves Ca2+ entry and Ca2+-release activated Ca2+ (CRAC) channels.

The current was evoked by UTP in separate MLS-9 cells with Ca2+-free bath solution (A), or with either 50 µM 2-APB (B) or 10 µM BTP2 (C) in the bath. D. The amplitude was quantified (as in Fig. 1E) and compared with standard bath solution. The number of cells is indicated on each bar. ***p<0.001

https://doi.org/10.1371/journal.pone.0062345.g003

We next asked whether CRAC and KCa3.1 channels contribute to the Ca2+ rise following P2Y receptor activation with UTP. None of the channel blockers affected the baseline Ca2+ level. When Ca2+ was omitted from the bath, UTP evoked only a rapidly rising Ca2+ transient due to release from internal stores and its peak amplitude was unchanged (Fig. 4A). The same response was seen with the blocker, 10 µM BTP2, which selectively blocks Ca2+ entry through CRAC channels. The secondary decay phase of the Ca2+ response was decreased by 50 µM 2-APB (Fig. 4A), as expected from its ability to block CRAC channels. The peak was also greatly decreased, which is not surprising because 2-APB was originally described as a membrane permeant inhibitor of the IP3 receptor [32] and is well known to reduce Ca2+ release from stores (reviewed in [33]). Interestingly, the KCa3.1 blocker, TRAM-34, reduced the secondary phase (Ca2+ entry) (Fig. 4B) but did not affect the initial peak due to Ca2+ release from stores. The SK3 blocker, apamin, had little or no effect. To compare the overall Ca2+ signal, the baseline was subtracted and the area under the curve was calculated for the first 4 min after UTP was added (Fig. 4C). Compared with untreated cells, the Ca2+ signal was dramatically reduced by 2-APB, and to a smaller degree by omitting Ca2+ or adding BTP2 or TRAM-34 (but not apamin) to the bath. With Ca2+-free bath solution, 2-APB further reduced the peak amplitude (340/380 ratio = 2.8±0.3; not shown) and area under the curve (to 145±15), consistent with its inhibition of Ca2+ release from stores.

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Figure 4. KCa3.1 activation promotes store-operated Ca2+ entry and refilling, and involves CRAC channels.

When used, the Ca2+-free solution or ion channel blocker (50 µM 2-APB, 10 µM BTP2, 1 µM TRAM-34, 100 nM apamin) was present in the bath throughout the recording period. A, B. Representative Fura-2 traces show the UTP-evoked Ca2+ signals from six MLS-9 cells on six separate coverslips. The same control cell is shown in A and B. The insets show the summarized peak responses for the number of cells indicated on each bar. ***p<0.001 C. Summary of the area under the curve (arbitrary units) calculated for the first 4 min of the response (same treatments as in A and B). D, E. Representative Fura-2 traces showing the first and second responses to UTP, with a 5-min recovery period between stimuli. The same control cell is shown in D and E. F. Summary comparing the maximal responses to the first and second UTP stimulus; i.e., Peak 2/Peak 1×100 (same treatments as in D and E). In panels C and F, the number of cells is indicated on each bar, and *p<0.05, **p<0.01, ***p<0.001

https://doi.org/10.1371/journal.pone.0062345.g004

To more directly analyze the role of CRAC and KCa3.1 channels in store refilling, we applied a second UTP treatment after a 5 min recovery period (examples in Fig. 4D, E; summary in Fig. 4F). In control cells, the second Ca2+ rise was substantial (Fig. 4D). On average, the peak reached 67.2±4.9% of the first response (Fig. 4F), indicating that 5 min was sufficient for considerable store refilling to occur. In contrast, the peak2/peak1 ratio was markedly reduced in the absence of Ca2+ (to 3.9±1.8% of the control level) or in the presence of 2-APB (14.1±4.1%), BTP2 (17.5±5.4%) or TRAM-34 (17.7±4.9%) in the bath. The response with BTP2 was essentially identical to that in the Ca2+ free bath, as expected for normal Ca2+ release from stores without influx. When Ca2+ was omitted from the bath, the already negligible second peak was unchanged by 2-APB or BTP2 (not shown). Again, apamin had no effect. Together, these data support the hypothesis that, following P2Y receptor activation, Ca2+ influx through CRAC/Orai1 channels replenishes the depleted stores, and this is facilitated by KCa3.1 (but not SK3) channel activity.

Evidence for a close proximity of KCa3.1 and CRAC/Orai1 channels

The previous results (Figs. 3, 4) show a functional coupling between Ca2+ influx through CRAC and KCa3.1 activation, and a reciprocal role for KCa3.1 in promoting Ca2+ entry and store refilling. The high global free Ca2+ concentration needed for KCa3.1 activation (Fig. 2) suggests that CRAC/Orai1 channels must be close to KCa3.1 channels in order for local Ca2+ to be high enough. A common test of proximity between a Ca2+ source and a responder molecule is to compare the effects of EGTA and BAPTA. While their Ca2+ affinities are similar at physiological pH, the binding rate constant for Ca2+ is 100–160 times faster for BAPTA (kon = 4.5×108 M−1s−1) than for EGTA (2.7×106 M−1s−1) [34]. In whole-cell recordings with the slower buffer, EGTA, the amplitude of the UTP-evoked KCa3.1 current was 358±41 pA at +80 mV (Fig. 1E). Using a BAPTA-containing pipette solution with the same concentration of free Ca2+ (120 nM), the baseline current in standard bath was small, and UTP activated a KCa3.1 current (compare Fig. 5A with Figs. 1, 2). This means that Ca2+ ions entering through CRAC channels could activate some KCa3.1 channels before being chelated. However, the average KCa3.1 amplitude was significantly smaller with BAPTA (214.1±41.4 pA) than with EGTA in the pipette solution (Fig. 5B). This provides biophysical evidence for a close proximity between KCa3.1 and CRAC channels.

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Figure 5. Evidence for a close proximity of KCa3.1 and CRAC/Orai1 channels.

A. A representative whole-cell recording from an MLS-9 microglia cell with internal Ca2+ buffered to 120 nM using 1 mM of the fast Ca2+ buffer, BAPTA. The two traces show currents before (control) and after 100 µM UTP was added to the bath. The voltage protocol was the same as in Figures 1 and 2; i.e., a voltage step to +50 mV was followed by a voltage ramp from −100 to +80 mV (holding potential, −70 mV). B. Comparison of the KCa3.1 current amplitude at +80 mV. Intracellular Ca2+ was buffered to 120 nM with either 1 mM EGTA or 1 mM BAPTA (*p<0.05, Student's t-test). C. High-magnification, deconvolved images of MLS-9 cells show immunolabeling for KCa3.1 (red), Orai1 (green), and the nuclear marker, DAPI (blue) (scale bar  = 10 µm). Below the main panels are magnifications of the two boxed areas in the merged image (scale bars = 2 µm).

https://doi.org/10.1371/journal.pone.0062345.g005

Next, immunocytochemistry was conducted to examine the subcellular distribution of KCa3.1 and Orai1 (CRAC) proteins in MLS-9 cells (Fig. 5C). Orai1 staining was widespread and punctate, as we recently found in primary rat microglia [11]. KCa3.1 showed widespread staining throughout the cell and at the surface, and not surprisingly, KCa3.1 and Orai1 proteins were closely associated, as seen in the two magnified regions (Fig. 5C). This is consistent with the patch-clamp results suggesting that KCa3.1 and Orai1 are physically close. Evidence of selective labeling is that negative controls were blank when the primary antibodies were omitted, and neither primary antibody revealed staining in the nucleus.

Roles for CRAC and KCa3.1 channels in microglia migration

Here, we show for the first time that transmigration of primary rat microglia is increased by P2Y receptor activation by UTP (i.e., more than a 3-fold increase; Fig. 6). [Note: we always use primary microglia for functional assays.]. Transmigration and the increased migration in response to UTP was reduced 89% by suramin. Together, this pharmacology implicates the P2Y2 receptor. Most notably, transmigration was strongly inhibited by the CRAC/Orai1 channel blockers, 2-APB (reduced by 84%) and BTP2 (reduced by 76%). In addition, there was a 55% inhibition by the KCa3.1 blocker, TRAM-34. The SK1–SK3 blocker, apamin, did not reduce migration. This pharmacological profile exactly parallels that of the UTP-induced Ca2+ signaling and activation of KCa3.1 channels (Figs. 1, 3, 4).

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Figure 6. Roles for CRAC and KCa3.1 channels in microglia migration.

Primary cultured rat microglia were seeded on filters with 8 µm-diameter pores and placed in the upper insert of TranswellTM chambers. After 24 h, transmigration was compared without (control) or with 100 µM UTP, in the lower chamber. The following antagonists were added to the microglia-containing upper well: the P2Y receptor antagonist, 100 µM suramin; blockers of CRAC/Orai1 (50 µM 2-APB, 10 µM BTP2), KCa3.1 (1 µM TRAM-34) or SK1–SK3 (100 nM apamin). For each treatment, cell counts were summed from 5 random fields of view at 20× magnification. The number of separate cell cultures is indicated on each bar. Statistical differences between control and UTP-treated cells (###p<0.001), and for UTP-treated cells with or without antagonists (***p<0.001) were determined by 1-way ANOVA with Tukey's post hoc test.

https://doi.org/10.1371/journal.pone.0062345.g006

Discussion

Microglial activation is multi-faceted, with diverse Ca2+-dependent functions that can orchestrate the inflammatory response to CNS injury. The specificity and accurate execution of microglial functions will depend on appropriately coupling external stimuli to Ca2+ signals and downstream effectors. Several G-protein coupled metabotropic purinergic receptors (P2Y2, P2Y4, P2Y6, P2Y12) have been identified in microglia (reviewed in [3], [7], [35], [36]). The use of agonists and antagonists can discriminate between them, and our results implicate P2Y2. That is, the UTP concentration used (100 µM) strongly activates P2Y2 and P2Y4 receptors, but only weakly activates P2Y6 [27], [37], [38]. The response was dramatically reduced by suramin at a concentration (100 µM) that fully inhibits P2Y2, inhibits P2Y 6 by ∼30%, and does not inhibit P2Y4 [27]. P2Y receptors elevate Ca2+ through IP3-mediated release from internal stores and influx through store-operated Ca2+ entry (SOCE). Here, UTP evoked a biphasic Ca2+ rise, with a rapid transient (typical of internal release) followed by a smaller plateau phase (typical of store-operated Ca2+ entry).

Following depletion of Ca2+ stores, rapid replenishment is important to prepare the cell for another stimulus; e.g., in cells with Ca2+ oscillations and during migration (reviewed in [39]). T lymphocyte activation is exemplary; i.e., the Ca2+ oscillations that are required to facilitate gene activation result from cyclical Ca2+ release from stores and subsequent refilling, which depends on CRAC/Orai1 (reviewed in [40]). There are multiple Ca2+ entry pathways in microglia (reviewed in [8], [41]), and in rat microglia, we previously found that the Ca2+-release-activated Ca2+ (CRAC/Orai1) channel is activated following store depletion (by thapsigargin) [10]. Here, we found that both the UTP-evoked Ca2+ plateau phase and the refilling of stores were mediated by Ca2+ influx through CRAC channels. Both processes were nearly abolished by omitting extracellular Ca2+, by the channel blocker, 2-APB and, importantly, by BTP2 at a concentration that is selective for CRAC/Orai1 channels [30], [31].

To maintain the driving force for optimal Ca2+ influx, a hyperpolarizing conductance is required. In microglia, depolarization reduced the Ca2+ rise after UTP stimulation [3], [9]. KCa3.1 channels perform this role during T cell activation ([42], [43]; reviewed in [40]) and in human macrophages [44]. Because both SK3 and KCa3.1 channels are expressed in primary rat microglia [12], [13], [45], and both currents are reliably activated (by riluzole) in MLS-9 cells [14], we had expected both to contribute in response to UTP. Surprisingly, only the KCa3.1 current was activated, and only KCa3.1 promoted the CRAC-mediated Ca2+ rise and refilling of stores. A reciprocal relation was seen, wherein KCa3.1 activation required Ca2+ influx and this was mediated by CRAC/Orai1 channels. Based on this functional coupling, we anticipated that KCa3.1 and Orai1 proteins would be in close proximity, and immunostaining showed that both were prevalent and widespread throughout MLS-9 cells. We recently reported a similar Orai1 distribution in primary rat microglia [11].

Not surprisingly, by elevating intracellular Ca2+, P2Y2 receptors can evoke Ca2+-activated K+ currents in some other cell types. For instance, UTP-stimulation of P2Y2 receptors activated KCa3.1 channels when exogenously co-expressed in Xenopus oocytes [46], and UTP can activate KCa3.1 in macrophages [44]. However, whether this involves a local trans-activation by specific Ca2+ channels is not known. Activation of KCa3.1 by nearby CRAC/Orai1 channels in microglia might reflect a specific coupling in non-excitable cells that do not express or use voltage-dependent Ca2+ channels (VDCCs). In endothelial cells, opening of TRPV4 channels evoked local Ca2+ “sparklets” that activated nearby small- and intermediate-conductance channels that were presumed to be KCa2.3 and KCa3.1 [47]. In some neurons, KCa2.x channels can be activated by nearby voltage-dependent Ca2+ channels (VDCCs), N-methyl d-aspartate (NMDA) receptors, and nicotinic acetylcholine receptors [48]. In cerebellar Purkinje cells, KCa3.1 channels interact with, and are activated by Cav3.2 VDCCs [49].

Purinergic receptors mediate numerous microglial functions. ATP is considered an important trigger for responses to acute injury, and it increases microglial motility and migration in vivo and in vitro ([6], [50], [51]; reviewed in [3], [7], [35], [36]). The focus has been on roles of P2X4 and P2Y12 receptors in chemotaxis, PLC-mediated rises in intracellular Ca2+, and translocation of β1 integrins [4], [5], [7]. However, P2X4 and P2Y12 receptors are not activated by UTP. We found that UTP increased migration of primary rat microglia, and the pharmacological profile clearly implicated P2Y2 receptors, just as we observed for the Ca2+ signaling and KCa3.1 channel activation. In P2Y2 receptor null mice, chemotaxis is impaired in neutrophils [52], monocytes and macrophages [53]. Cell migration is regulated by Ca2+ signals that range from transient localized ‘flickers’ to oscillations and sustained gradients [54][57]. In some cells, Ca2+ oscillations produce optimal migration [58] but there is limited information about the specific Ca2+-permeable channels involved. The TRPM7 channel was implicated in Ca2+ flicker activity during migration in a neuroblastoma cell line transfected with this channel [56]. SKF96365, a drug that blocks several Ca2+ permeable channels including TRPM7 and CRAC/Orai1, reduced migration of a breast tumor cell line [59]. Reduced migration was seen in neutrophils from heterozygous Orai1 knockout mice and in the HL-60 myeloid cell line after siRNA-mediated Orai1 depletion [60]. Not surprisingly, considering the roles of CRAC/Orai1 and KCa3.1 channels in UTP-evoked Ca2+ entry and store refilling, we found that these channels contribute to UTP-stimulated chemotaxis of primary rat microglia. We recently discovered that migrating rat microglia possess podosomes, which are tiny multi-molecular structures with dual functions in mediating cell adhesion and substrate degradation [11], [26]. Interestingly, the podosomes are enriched in Orai1 (and several Ca2+-dependent proteins), and blocking Ca2+ entry through CRAC/Orai1 channels inhibited podosome formation and migration [11]. KCa3.1 is expressed in several migratory cell types, and pharmacology implicates it in migration (reviewed in [61][63]. For instance, lysophosphatidic acid-stimulated chemotaxis was inhibited by charybdotoxin and clotrimazole [64], which are less selective KCa3.1 blockers than TRAM-34. Further studies will be needed to determine whether KCa3.1 and CRAC/Orai1 act in concert to facilitate UTP-stimulated microglial migration by promoting specific downstream processes, including podosome formation.

Two surprising results were that only KCa3.1 (not SK3) was activated by UTP, and channel activation was remarkably insensitive to simply elevating Ca2+ in the intracellular (pipette) solution. The EC50 was 7.6 µM Ca2+ and no current was seen at 2.5 µM Ca2+. The UTP-evoked Ca2+ rise peaked at 5.3 µM in the whole cell but is undoubtedly higher adjacent to open CRAC channels. While a range of EC50 values has been reported for activating KCa3.1 channels, they are well below 1 µM Ca2+ (reviewed in [65][67]). For instance, reports on lymphocytes indicate a threshold of about 200 nM Ca2+, an EC50 of 300–450 nM, and saturation at 1 µM [43], [68], [69]. For cloned KCa3.1 channels, the expression system might affect the Ca2+ sensitivity; e.g., an EC50 of 95 nM Ca2+ was seen in CHO cells [70] versus 700 nM in Xenopus oocytes [71]. The biological basis for these differences is unknown. While we do not know the reasons for the very high EC50 for activating KCa3.1 or the failure to activate SK3 channels in the present study, it is worth considering the known mechanism for activating these channels.

SK and KCa3.1 channels are tetramers and are activated by Ca2+ binding to calmodulin, which is bound to the CaM-binding domain (CaMBD) in the proximal C-terminus of each channel monomer [43], [71], [72]. Each CaM molecule has four E-F hands that can potentially bind Ca2+; two each in the C- and N-lobes, which are connected by a flexible linker region [73]. Only one E-F hand in the N-lobe is apparently required for the Ca2+-dependent gating of SK channels and this produces a Hill coefficient of ∼4 in the Ca2+-dose-response curve [73], [74]. For KCa3.1, Hill coefficients of 3.9 [68], 3.2 [70], and 4.6 (present study) have been reported. Thus, it is unlikely that the low Ca2+ sensitivity in this study reflects fewer functional Ca2+ binding sites. The selective activation of KCa3.1 but not SK3 is intriguing because we recently found that the neuroprotective drug, riluzole, reliably activates both channels in MLS-9 cells [14]. For heterologously expressed channels, riluzole shifts the Ca2+ dependence to the left, thereby increasing the probability of channel opening at lower Ca2+ levels. Riluzole reduced the EC50 from 470 to 112 nM Ca2+ for expressed rat SK2 [15], activated rat SK3 at 100 nM intracellular Ca2+ [75], and increased the current amplitude by 30-fold at 250 nM Ca2+ for human SK3 and KCa3.1 channels [76]. The mechanism for riluzole activation of SK3 and KCa3.1 must be different in MLS-9 cells because micromolar levels of Ca2+ alone did not activate the currents (present study), and riluzole elevated Ca2+ only to 200 nM [14]. One possibility is that P2Y2 receptor activation affects an unidentified accessory molecule that aids in channel activation.

For SK2 and SK3 channels, Ca2+ sensitivity is affected by CaM phosphorylation by CK2 protein kinase and PP2A protein phosphatase, which bind to the channels [77], [78]. Thus, it is worth considering what is known about factors that regulate the Ca2+-sensitivity of KCa3.1 channels. While some studies show modulation by ATP in the intracellular solution, there is some conflicting data. The EC50 for channel activation in transfected oocytes was 490 nM Ca2+ without ATP and 320 nM with ATP [79]. For endogenous KCa3.1 channels in rat submandibular acinar cells, the Kd was 1.35 µM without ATP and 0.66 µM with ATP [80]. These small ATP effects cannot account for the high Kd (7.6 µM Ca2+ with ATP always present) in our study of KCa3.1 in microglia. KCa3.1 regulation might be cell-type specific. For instance, our early study suggested that CaMKII regulates the endogenous KCa3.1 channel in T cells but not the expressed channel in CHO cells [43]. Two studies showed that activation of KCa3.1 by hydrolyzable ATP analogues occurred with no change in Ca2+ sensitivity [81] and that channel activation was due to PKA in Xenopus oocytes (transfected) and in the T84 cell line (non-transfected) but not in transfected HEK cells [82]. However, another study of KCa3.1-transfected oocytes concluded that PKA inhibits the channels, and is independent of mechanisms controlling Ca2+ sensitivity [83]. While KCa3.1 channels interact with, and are regulated by some kinases and phosphatases (for an excellent recent review, see [84]), there is no evidence that they can modulate the Ca2+ dependence to account for the low sensitivity of the microglial KCa3.1 channel. AMP-activated protein kinase (AMPK) inhibits the current and directly binds to the distal C-terminus of the KCa3.1 protein [85]. The reported regulation by PKC is likely indirect, and was not affected by mutating the PKC consensus sites [86]. Recent discoveries concerning KCa3.1 regulation have begun to identify interacting proteins. The lipid PI3P phosphatase, myotubularin-related protein 6 (MTMR6), interacts with KCa3.1 and inhibits its function by dephosphorylating PI3P near the channel [87]. The histidine kinase, nucleoside diphosphate kinase B (NDPK-B) binds to and activates KCa3.1 [88]; an effect that is reversed by protein histidine phosphatase (PHPT-1) [89].

A recent study found that CaM-CaMBD interactions change the CaM conformation and increase its Ca2+ affinity [73]. While numerous SK1–SK3 splice variants have been found (some differing in the C-terminus that contains the CaMBD) (reviewed in [90]), very little is known about their Ca2+ sensitivities. Most relevant is the recent discovery of an SK2 variant with three extra amino acids in the CaMBD [73]. It has a reduced Ca2+ sensitivity, with an EC50 of 1 µM rather than ∼300 nM, but no change in the Hill coefficient. Three KCa3.1 variants have been found in rat colon: KCNN4a, KCNN4b and KCNN4c encode proteins of 425, 424, and 395 amino acids, respectively [91]. KCNN4b lacks a glutamine at position 415, and KCNN4c lacks the S2 transmembrane segment, but Ca2+ sensitivities were not examined. A dominant-negative variant found in lymphoid tissues lacks the N-terminus, and because it suppresses normal membrane KCa3.1 expression [92], is unlikely to account for the present results. Further studies will be needed to address whether microglia express a KCa3.1 channel splice variant that is less sensitive to Ca2+.

This work has broader implications because KCa3.1 channels are expressed in numerous cell types (mainly non-excitable), and have been implicated in a range of cell functions, as extensively reviewed in recent years [65], [84], [93][98]. For instance, initially described from studies of red blood cell volume regulation, KCa3.1 is now known to regulate activation of subsets of T lymphocytes, mediate salt and water transport across epithelia, regulate endothelial cell contributions to vascular tone, and modulate cell proliferation and differentiation of several cell types. There is less known about KCa3.1 in the CNS and it was initially thought to be absent from the brain [99]. KCa3.1 is present in microglia [45], [100], and we showed it is involved in p38 MAPK activation and subsequent superoxide and nitric oxide production [12], [45]. Blocking KCa3.1 with TRAM-34 reduced the ability of microglia to kill neurons in vitro and decreased retinal ganglion cell degeneration in vivo [12]. KCa3.1 is being considered as a clinical target for multiple diseases, from sickle cell anemia to inflammation, gastrointestinal disorders, heart disease, multiple sclerosis and stroke. Thus, there is interest in cell-specific mechanisms that control channel activation, Ca2+ sensitivity, and coupling to specific receptors and channels.

Acknowledgments

We thank Dr. Starlee Lively for advice on the transmigration assay, Dr. Baosong Liu for helpful technical advice on patch clamping and measuring Ca2+, and Xiaoping Zhu for assistance with cell cultures.

Author Contributions

Obtained funding, supervised RF and technician: LS. Conceived and designed the experiments: LS RF. Performed the experiments: RF. Analyzed the data: RF LS. Wrote the paper: LS RF.

References

  1. 1. Hanisch UK, Kettenmann H (2007) Microglia: active sensor and versatile effector cells in the normal and pathologic brain. Nat Neurosci 10: 1387–1394.
  2. 2. Inoue K (2002) Microglial activation by purines and pyrimidines. Glia 40: 156–163.
  3. 3. Farber K, Kettenmann H (2006) Purinergic signaling and microglia. Pflugers Arch 452: 615–621.
  4. 4. Hidetoshi T-S, Makoto T, Inoue K (2012) P2Y receptors in microglia and neuroinflammation. WIREs Membr Transp Signal 1: 493–501.
  5. 5. Haynes SE, Hollopeter G, Yang G, Kurpius D, Dailey ME, et al. (2006) The P2Y12 receptor regulates microglial activation by extracellular nucleotides. Nat Neurosci 9: 1512–1519.
  6. 6. Honda S, Sasaki Y, Ohsawa K, Imai Y, Nakamura Y, et al. (2001) Extracellular ATP or ADP induce chemotaxis of cultured microglia through Gi/o-coupled P2Y receptors. J Neurosci 21: 1975–1982.
  7. 7. Ohsawa K, Kohsaka S (2011) Dynamic motility of microglia: purinergic modulation of microglial movement in the normal and pathological brain. Glia 59: 1793–1799.
  8. 8. Farber K, Kettenmann H (2006) Functional role of calcium signals for microglial function. Glia 54: 656–665.
  9. 9. McLarnon JG (2005) Purinergic mediated changes in Ca2+ mobilization and functional responses in microglia: effects of low levels of ATP. J Neurosci Res 81: 349–356.
  10. 10. Ohana L, Newell EW, Stanley EF, Schlichter LC (2009) The Ca2+ release-activated Ca2+ current (ICRAC) mediates store-operated Ca2+ entry in rat microglia. Channels (Austin) 3: 129–139.
  11. 11. Siddiqui TA, Lively S, Vincent C, Schlichter LC (2012) Regulation of podosome formation, microglial migration and invasion by Ca2+-signaling molecules expressed in podosomes. J Neuroinflammation 9: 250.
  12. 12. Kaushal V, Koeberle PD, Wang Y, Schlichter LC (2007) The Ca2+-activated K+ channel KCNN4/KCa3.1 contributes to microglia activation and nitric oxide-dependent neurodegeneration. J Neurosci 27: 234–244.
  13. 13. Schlichter LC, Kaushal V, Moxon-Emre I, Sivagnanam V, Vincent C (2010) The Ca2+ activated SK3 channel is expressed in microglia in the rat striatum and contributes to microglia-mediated neurotoxicity in vitro. J Neuroinflammation 7: 4.
  14. 14. Liu BS, Ferreira R, Lively S, Schlichter LC (2012) Microglial SK3 and SK4 currents and activation state are modulated by the neuroprotective drug, riluzole. J Neuroimmune Pharmacol
  15. 15. Cao YJ, Dreixler JC, Couey JJ, Houamed KM (2002) Modulation of recombinant and native neuronal SK channels by the neuroprotective drug riluzole. Eur J Pharmacol 449: 47–54.
  16. 16. Sivagnanam V, Zhu X, Schlichter LC (2010) Dominance of E. coli phagocytosis over LPS in the inflammatory response of microglia. J Neuroimmunol 227: 111–119.
  17. 17. Zhou W, Cayabyab FS, Pennefather PS, Schlichter LC, DeCoursey TE (1998) HERG-like K+ channels in microglia. J Gen Physiol 111: 781–794.
  18. 18. Cayabyab FS, Khanna R, Jones OT, Schlichter LC (2000) Suppression of the rat microglia Kv1.3 current by src-family tyrosine kinases and oxygen/glucose deprivation. Eur J Neurosci 12: 1949–1960.
  19. 19. Cayabyab FS, Schlichter LC (2002) Regulation of an ERG K+ current by Src tyrosine kinase. J Biol Chem 277: 13673–13681.
  20. 20. Cayabyab FS, Tsui FW, Schlichter LC (2002) Modulation of the ERG K+ current by the tyrosine phosphatase, SHP-1. J Biol Chem 277: 48130–48138.
  21. 21. Schlichter LC, Mertens T, Liu B (2011) Swelling activated Cl- channels in microglia: Biophysics, pharmacology and role in glutamate release. Channels (Austin) 5: 128–137.
  22. 22. Newell EW, Schlichter LC (2005) Integration of K+ and Cl currents regulate steady-state and dynamic membrane potentials in cultured rat microglia. J Physiol 567: 869–890.
  23. 23. Schlichter LC, Sakellaropoulos G, Ballyk B, Pennefather PS, Phipps DJ (1996) Properties of K+ and Cl channels and their involvement in proliferation of rat microglial cells. Glia 17: 225–236.
  24. 24. Jiang X, Newell EW, Schlichter LC (2003) Regulation of a TRPM7-like current in rat brain microglia. J Biol Chem 278: 42867–42876.
  25. 25. Grynkiewicz G, Poenie M, Tsien RY (1985) A new generation of Ca2+ indicators with greatly improved fluorescence properties. J Biol Chem 260: 3440–3450.
  26. 26. Vincent C, Siddiqui TA, Schlichter LC (2012) Podosomes in migrating microglia: components and matrix degradation. J Neuroinflammation 9: 190.
  27. 27. von Kugelgen I (2006) Pharmacological profiles of cloned mammalian P2Y-receptor subtypes. Pharmacol Ther 110: 415–432.
  28. 28. Parekh AB (2010) Store-operated CRAC channels: function in health and disease. Nat Rev Drug Discov 9: 399–410.
  29. 29. Peinelt C, Lis A, Beck A, Fleig A, Penner R (2008) 2-Aminoethoxydiphenyl borate directly facilitates and indirectly inhibits STIM1-dependent gating of CRAC channels. J Physiol 586: 3061–3073.
  30. 30. He LP, Hewavitharana T, Soboloff J, Spassova MA, Gill DL (2005) A functional link between store-operated and TRPC channels revealed by the 3,5-bis(trifluoromethyl)pyrazole derivative, BTP2. J Biol Chem 280: 10997–11006.
  31. 31. Takezawa R, Cheng H, Beck A, Ishikawa J, Launay P, et al. (2006) A pyrazole derivative potently inhibits lymphocyte Ca2+ influx and cytokine production by facilitating transient receptor potential melastatin 4 channel activity. Mol Pharmacol 69: 1413–1420.
  32. 32. Maruyama T, Kanaji T, Nakade S, Kanno T, Mikoshiba K (1997) 2APB, 2-aminoethoxydiphenyl borate, a membrane-penetrable modulator of Ins(1,4,5)P3-induced Ca2+ release. J Biochem 122: 498–505.
  33. 33. DeHaven WI, Smyth JT, Boyles RR, Bird GS, Putney JW Jr (2008) Complex actions of 2-aminoethyldiphenyl borate on store-operated calcium entry. J Biol Chem 283: 19265–19273.
  34. 34. Tsien RY (1980) New calcium indicators and buffers with high selectivity against magnesium and protons: design, synthesis, and properties of prototype structures. Biochemistry 19: 2396–2404.
  35. 35. Gyoneva S, Orr AG, Traynelis SF (2009) Differential regulation of microglial motility by ATP/ADP and adenosine. Parkinsonism Relat Disord 15 Suppl 3S195–199.
  36. 36. Inoue K (2008) Purinergic systems in microglia. Cell Mol Life Sci 65: 3074–3080.
  37. 37. Jacobson KA, Boeynaems JM (2010) P2Y nucleotide receptors: promise of therapeutic applications. Drug Discov Today 15: 570–578.
  38. 38. Jacobson KA, Ivanov AA, de Castro S, Harden TK, Ko H (2009) Development of selective agonists and antagonists of P2Y receptors. Purinergic Signal 5: 75–89.
  39. 39. Parekh AB, Putney JW Jr (2005) Store-operated calcium channels. Physiol Rev 85: 757–810.
  40. 40. Prakriya M, Lewis RS (2003) CRAC channels: activation, permeation, and the search for a molecular identity. Cell Calcium 33: 311–321.
  41. 41. Moller T (2002) Calcium signaling in microglial cells. Glia 40: 184–194.
  42. 42. Fanger CM, Rauer H, Neben AL, Miller MJ, Rauer H, et al. (2001) Calcium-activated potassium channels sustain calcium signaling in T lymphocytes. Selective blockers and manipulated channel expression levels. J Biol Chem 276: 12249–12256.
  43. 43. Khanna R, Chang MC, Joiner WJ, Kaczmarek LK, Schlichter LC (1999) hSK4/hIK1, a calmodulin-binding KCa channel in human T lymphocytes. Roles in proliferation and volume regulation. J Biol Chem 274: 14838–14849.
  44. 44. Gao YD, Hanley PJ, Rinne S, Zuzarte M, Daut J (2010) Calcium-activated K+ channel (KCa3.1) activity during Ca2+ store depletion and store-operated Ca2+ entry in human macrophages. Cell Calcium 48: 19–27.
  45. 45. Khanna R, Roy L, Zhu X, Schlichter LC (2001) K+ channels and the microglial respiratory burst. Am J Physiol Cell Physiol 280: C796–806.
  46. 46. Hede SE, Amstrup J, Klaerke DA, Novak I (2005) P2Y2 and P2Y4 receptors regulate pancreatic Ca2+-activated K+ channels differently. Pflugers Arch 450: 429–436.
  47. 47. Sonkusare SK, Bonev AD, Ledoux J, Liedtke W, Kotlikoff MI, et al. (2012) Elementary Ca2+ signals through endothelial TRPV4 channels regulate vascular function. Science 336: 597–601.
  48. 48. Adelman JP, Maylie J, Sah P (2012) Small-conductance Ca2+-activated K+ channels: form and function. Annu Rev Physiol 74: 245–269.
  49. 49. Engbers JD, Anderson D, Asmara H, Rehak R, Mehaffey WH, et al. (2012) Intermediate conductance calcium-activated potassium channels modulate summation of parallel fiber input in cerebellar Purkinje cells. Proc Natl Acad Sci U S A 109: 2601–2606.
  50. 50. Kurpius D, Nolley EP, Dailey ME (2007) Purines induce directed migration and rapid homing of microglia to injured pyramidal neurons in developing hippocampus. Glia 55: 873–884.
  51. 51. Yao J, Harvath L, Gilbert DL, Colton CA (1990) Chemotaxis by a CNS macrophage, the microglia. J Neurosci Res 27: 36–42.
  52. 52. Chen Y, Corriden R, Inoue Y, Yip L, Hashiguchi N, et al. (2006) ATP release guides neutrophil chemotaxis via P2Y2 and A3 receptors. Science 314: 1792–1795.
  53. 53. Elliott MR, Chekeni FB, Trampont PC, Lazarowski ER, Kadl A, et al. (2009) Nucleotides released by apoptotic cells act as a find-me signal to promote phagocytic clearance. Nature 461: 282–286.
  54. 54. Brundage RA, Fogarty KE, Tuft RA, Fay FS (1991) Calcium gradients underlying polarization and chemotaxis of eosinophils. Science 254: 703–706.
  55. 55. Komuro H, Rakic P (1998) Orchestration of neuronal migration by activity of ion channels, neurotransmitter receptors, and intracellular Ca2+ fluctuations. J Neurobiol 37: 110–130.
  56. 56. Wei C, Wang X, Chen M, Ouyang K, Song LS, et al. (2009) Calcium flickers steer cell migration. Nature 457: 901–905.
  57. 57. Wei C, Wang X, Zheng M, Cheng H (2012) Calcium gradients underlying cell migration. Curr Opin Cell Biol 24: 254–261.
  58. 58. Schwab A, Schuricht B, Seeger P, Reinhardt J, Dartsch PC (1999) Migration of transformed renal epithelial cells is regulated by K+ channel modulation of actin cytoskeleton and cell volume. Pflugers Arch 438: 330–337.
  59. 59. Yang S, Zhang JJ, Huang XY (2009) Orai1 and STIM1 are critical for breast tumor cell migration and metastasis. Cancer Cell 15: 124–134.
  60. 60. Schaff UY, Dixit N, Procyk E, Yamayoshi I, Tse T, et al. (2010) Orai1 regulates intracellular calcium, arrest, and shape polarization during neutrophil recruitment in shear flow. Blood 115: 657–666.
  61. 61. Schmidt EM, Munzer P, Borst O, Kraemer BF, Schmid E, et al. (2011) Ion channels in the regulation of platelet migration. Biochem Biophys Res Commun 415: 54–60.
  62. 62. Schwab A, Nechyporuk-Zloy V, Gassner B, Schulz C, Kessler W, et al. (2011) Dynamic redistribution of calcium sensitive potassium channels (hKCa3.1) in migrating cells. J Cell Physiol 227: 686–696.
  63. 63. Schwab A, Wulf A, Schulz C, Kessler W, Nechyporuk-Zloy V, et al. (2006) Subcellular distribution of calcium-sensitive potassium channels (IK1) in migrating cells. J Cell Physiol 206: 86–94.
  64. 64. Schilling T, Stock C, Schwab A, Eder C (2004) Functional importance of Ca2+-activated K+ channels for lysophosphatidic acid-induced microglial migration. Eur J Neurosci 19: 1469–1474.
  65. 65. Jensen BS, Strobaek D, Olesen SP, Christophersen P (2001) The Ca2+-activated K+ channel of intermediate conductance: a molecular target for novel treatments? Curr Drug Targets 2: 401–422.
  66. 66. Pedarzani P, Stocker M (2008) Molecular and cellular basis of small- and intermediate-conductance, calcium-activated potassium channel function in the brain. Cell Mol Life Sci 65: 3196–3217.
  67. 67. Wulff H, Zhorov BS (2008) K+ channel modulators for the treatment of neurological disorders and autoimmune diseases. Chem Rev 108: 1744–1773.
  68. 68. Grissmer S, Nguyen AN, Cahalan MD (1993) Calcium-activated potassium channels in resting and activated human T lymphocytes. Expression levels, calcium dependence, ion selectivity, and pharmacology. J Gen Physiol 102: 601–630.
  69. 69. Mahaut-Smith MP, Schlichter LC (1989) Ca2+-activated K+ channels in human B lymphocytes and rat thymocytes. J Physiol 415: 69–83.
  70. 70. Joiner WJ, Wang LY, Tang MD, Kaczmarek LK (1997) hSK4, a member of a novel subfamily of calcium-activated potassium channels. Proc Natl Acad Sci U S A 94: 11013–11018.
  71. 71. Kohler M, Hirschberg B, Bond CT, Kinzie JM, Marrion NV, et al. (1996) Small-conductance, calcium-activated potassium channels from mammalian brain. Science 273: 1709–1714.
  72. 72. Xia XM, Fakler B, Rivard A, Wayman G, Johnson-Pais T, et al. (1998) Mechanism of calcium gating in small-conductance calcium-activated potassium channels. Nature 395: 503–507.
  73. 73. Zhang M, Abrams C, Wang L, Gizzi A, He L, et al. (2012) Structural basis for calmodulin as a dynamic calcium sensor. Structure 20: 911–923.
  74. 74. Keen JE, Khawaled R, Farrens DL, Neelands T, Rivard A, et al. (1999) Domains responsible for constitutive and Ca2+-dependent interactions between calmodulin and small conductance Ca2+-activated potassium channels. J Neurosci 19: 8830–8838.
  75. 75. Grunnet M, Jespersen T, Angelo K, Frokjaer-Jensen C, Klaerke DA, et al. (2001) Pharmacological modulation of SK3 channels. Neuropharmacology 40: 879–887.
  76. 76. Sankaranarayanan A, Raman G, Busch C, Schultz T, Zimin PI, et al. (2009) Naphtho[1,2-d]thiazol-2-ylamine (SKA-31), a new activator of KCa2 and KCa3.1 potassium channels, potentiates the endothelium-derived hyperpolarizing factor response and lowers blood pressure. Mol Pharmacol 75: 281–295.
  77. 77. Allen D, Fakler B, Maylie J, Adelman JP (2007) Organization and regulation of small conductance Ca2+-activated K+ channel multiprotein complexes. J Neurosci 27: 2369–2376.
  78. 78. Bildl W, Strassmaier T, Thurm H, Andersen J, Eble S, et al. (2004) Protein kinase CK2 is coassembled with small conductance Ca2+-activated K+ channels and regulates channel gating. Neuron 43: 847–858.
  79. 79. von Hahn T, Thiele I, Zingaro L, Hamm K, Garcia-Alzamora M, et al. (2001) Characterisation of the rat SK4/IK1 K+ channel. Cell Physiol Biochem 11: 219–230.
  80. 80. Hayashi M, Kunii C, Takahata T, Ishikawa T (2004) ATP-dependent regulation of SK4/IK1-like currents in rat submandibular acinar cells: possible role of cAMP-dependent protein kinase. Am J Physiol Cell Physiol 286: C635–646.
  81. 81. Gerlach AC, Gangopadhyay NN, Devor DC (2000) Kinase-dependent regulation of the intermediate conductance, calcium-dependent potassium channel, hIK1. J Biol Chem 275: 585–598.
  82. 82. Gerlach AC, Syme CA, Giltinan L, Adelman JP, Devor DC (2001) ATP-dependent activation of the intermediate conductance, Ca2+-activated K+ channel, hIK1, is conferred by a C-terminal domain. J Biol Chem 276: 10963–10970.
  83. 83. Neylon CB, D'Souza T, Reinhart PH (2004) Protein kinase A inhibits intermediate conductance Ca2+-activated K+ channels expressed in Xenopus oocytes. Pflugers Arch 448: 613–620.
  84. 84. Balut CM, Hamilton KL, Devor DC (2012) Trafficking of intermediate (KCa3.1) and small (KCa2.x) conductance, Ca2+-activated K+ channels: a novel target for medicinal chemistry efforts? ChemMedChem 7: 1741–1755.
  85. 85. Klein H, Garneau L, Trinh NT, Prive A, Dionne F, et al. (2009) Inhibition of the KCa3.1 channels by AMP-activated protein kinase in human airway epithelial cells. Am J Physiol Cell Physiol 296: C285–295.
  86. 86. Wulf A, Schwab A (2002) Regulation of a calcium-sensitive K+ channel (cIK1) by protein kinase C. J Membr Biol. 187: 71–79.
  87. 87. Srivastava S, Li Z, Lin L, Liu G, Ko K, et al. (2005) The phosphatidylinositol 3-phosphate phosphatase myotubularin- related protein 6 (MTMR6) is a negative regulator of the Ca2+-activated K+ channel KCa3.1. Mol Cell Biol 25: 3630–3638.
  88. 88. Srivastava S, Li Z, Ko K, Choudhury P, Albaqumi M, et al. (2006) Histidine phosphorylation of the potassium channel KCa3.1 by nucleoside diphosphate kinase B is required for activation of KCa3.1 and CD4 T cells. Mol Cell 24: 665–675.
  89. 89. Srivastava S, Zhdanova O, Di L, Li Z, Albaqumi M, et al. (2008) Protein histidine phosphatase 1 negatively regulates CD4 T cells by inhibiting the K+ channel KCa3.1. Proc Natl Acad Sci U S A 105: 14442–14446.
  90. 90. Faber ES (2009) Functions and modulation of neuronal SK channels. Cell Biochem Biophys 55: 127–139.
  91. 91. Barmeyer C, Rahner C, Yang Y, Sigworth FJ, Binder HJ, et al. (2010) Cloning and identification of tissue-specific expression of KCNN4 splice variants in rat colon. Am J Physiol Cell Physiol 299: C251–263.
  92. 92. Ohya S, Niwa S, Yanagi A, Fukuyo Y, Yamamura H, et al. (2011) Involvement of dominant-negative spliced variants of the intermediate conductance Ca2+-activated K+ channel, KCa3.1, in immune function of lymphoid cells. J Biol Chem 286: 16940–16952.
  93. 93. Cahalan MD, Chandy KG (2009) The functional network of ion channels in T lymphocytes. Immunol Rev 231: 59–87.
  94. 94. Edwards G, Feletou M, Weston AH (2010) Endothelium-derived hyperpolarising factors and associated pathways: a synopsis. Pflugers Arch 459: 863–879.
  95. 95. Grgic I, Kaistha BP, Hoyer J, Kohler R (2009) Endothelial Ca2+-activated K+ channels in normal and impaired EDHF-dilator responses--relevance to cardiovascular pathologies and drug discovery. Br J Pharmacol 157: 509–526.
  96. 96. Kohler R, Kaistha BP, Wulff H (2010) Vascular KCa-channels as therapeutic targets in hypertension and restenosis disease. Expert Opin Ther Targets 14: 143–155.
  97. 97. Lam J, Wulff H (2011) The Lymphocyte Potassium Channels Kv1.3 and KCa3.1 as Targets for Immunosuppression. Drug Dev Res 72: 573–584.
  98. 98. Wulff H, Kolski-Andreaco A, Sankaranarayanan A, Sabatier JM, Shakkottai V (2007) Modulators of small- and intermediate-conductance calcium-activated potassium channels and their therapeutic indications. Curr Med Chem 14: 1437–1457.
  99. 99. Bond CT, Maylie J, Adelman JP (2005) SK channels in excitability, pacemaking and synaptic integration. Curr Opin Neurobiol 15: 305–311.
  100. 100. Eder C (2010) Ion channels in monocytes and microglia/brain macrophages: promising therapeutic targets for neurological diseases. J Neuroimmunol 224: 51–55.