Mesenchymal stromal cells (MSCs) from different sources represent a heterogeneous population of proliferating non-differentiated cells that contain multipotent stem cells capable of originating a variety of mesenchymal cell lineages. By using Ca2+ imaging and the Ca2+ dye Fluo-4, we studied MSCs from the human adipose tissue and examined Ca2+ signaling initiated by a variety of GPCR ligands, focusing primarily on adrenergic and purinergic agonists. Being characterized by a relative change of Fluo-4 fluorescence, agonist-induced Ca2+ responses were generated in an “all-or-nothing” fashion. Specifically, at relatively low doses, agonists elicited undetectable responses but initiated quite similar Ca2+ transients at all concentrations above the threshold. The inhibitory analysis and Ca2+/IP3 uncaging pointed at the phosphoinositide cascade as a pivotal pathway responsible for agonist transduction and implicated Ca2+-induced Ca2+ release (CICR) in shaping agonists-dependent Ca2+ signals. Altogether, our data suggest that agonist transduction in MSCs includes two fundamentally different stages: an agonist initially triggers a local, gradual, and relatively small Ca2+ signal, which next stimulates CICR to accomplish transduction with a large and global Ca2+ transient. By involving the trigger-like mechanism CICR, a cell is capable of generating Ca2+ responses of virtually universal shape and magnitude at different agonist concentrations above the threshold.
- Ca2+ signaling
- G-protein coupled receptors
- calcium-induced calcium release
- IP3 receptors
- mesenchymal stromal cells
- adipose tissue
Mesenchymal stromal cells (MSCs) are described as a heterogeneous cellular pool that includes immature cells responsible for the replenishment of supportive and connective tissues due to their capability of maintaining self-renewal and multipotent differentiation [1, 2, 3]. By unique biologic properties, cultured MSCs from different sources attract sufficient interest in the fields of regenerative medicine and immunotherapy [4, 5, 6]. Despite evident progress in MSC biology spurred by the therapeutic potential of these cells, current knowledge on their receptor and signaling systems remains scarce. Evidence exists that MSCs are capable of sensing complex extracellular cues, including hormones, cytokines, and nucleotides [7, 8]. This implies that MSCs employ multiple surface receptors and signaling pathways to adjust their physiological functions to specific tissue microenvironment.
Here, we studied MSCs derived from the human adipose tissue and examined Ca2+ signaling initiated by a variety of agonists of G-protein coupled receptors (GPCRs). We specifically focused on adrenergic and purinergic signaling systems that attracted us for the following reasons. It has been known for a long time that noradrenaline released by sympathetic nerves regulates distinct physiological processes in the adipose tissue such as lipid and glucose metabolism and secretion of distinct signaling molecules, including adipocytokines and cytokines . Hence, MSCs that reside in the adipose tissue can be subjected to the action of noradrenaline and factors released by adipocytes on adrenergic stimulation. Purinergic agonists have been documented as an important factor determining MSC fate [7, 8, 10, 11, 12]. Reportedly, ATP serves both as an adipogenic regulator and an osteogenic factor, while its downstream product adenosine switches off adipogenic differentiation and promotes osteogenesis [13, 14]. Damaged tissues are an abundant source of extracellular ATP that may be converted by extracellular nucleotidases to ADP and eventually to adenosine . It therefore might be expected that MSCs are exposed to and regulated by nucleotides and adenosine when these cells migrate
The responsiveness to purines and pyrimidines is widespread among eukaryotic cells, which express numerous purinoreceptors from the P1 and P2 families. The P1 subgroup includes four G-protein-coupled receptors (A1, A2A, A2B, A3) recognizing adenosine as an endogenous agonist . The more diverse P2 family is composed of ionotropic P2X and metabotropic P2Y receptors. P2X receptors are cationic channels specifically gated by ATP, while P2Y receptors are activated by multiple purine and pyrimidine nucleotides or by sugar nucleotides and couple to intracellular second messenger pathways by heteromeric G proteins [17, 18]. In mammals, seven genes encode P2X subunits (P2X1–7) that can form homo- and heterotrimeric cation channels with noticeable Ca2+ permeability [19, 20]. The P2Y subfamily includes eight members (P2Y1,2,4,6,11,12,13,14), which are distinct by ligand specificity and coupling to downstream signaling pathways, including the ubiquitous phosphoinositide cascade [17, 18].
Nine genes encode human adrenoreceptors, which all belong to the GPCR superfamily and compose three distinctive subgroups, including three α1 (α1A, α1B, α1D), three α2 (α2A, α2B, α2C), and three β (β1, β2, β3) receptor subtypes. Canonically, α1-adrenoreceptors couple to Gq and are ubiquitously involved in Ca2+ signaling . Although α2 isoforms widely regulate adenylyl cyclase via Gi, their coupling to phospholipase C (PLC) and Ca2+ mobilization has also been documented . All three β-subtypes are linked to adenylyl cyclase by Gs, although β2 and β3 also couple to Gi, and directly do not control intracellular Ca2+ . Given that certain isoforms of adrenergic and purinergic receptors are coupled to Ca2+ mobilization in diverse cell types, we considered Ca2+ imaging as an adequate approach to detail purinergic and adrenergic transduction in MSCs.
2. Materials and methods
2.1. Cell isolation and culturing
MSCs of the first passage were obtained from the Faculty of Basic Medicine at Lomonosov Moscow State University. All procedures that involved human participants were performed in accordance with the ethical standards approved by the Bioethical Committee of the Faculty based on the 1964 Helsinki declaration and its later amendments. The study involved 21 healthy (not suffered from infectious or systemic diseases and malignancies) individuals from 21 to 55 years old, and informed consent was obtained from each participant.
Cells were isolated from subcutaneous fat tissue of healthy donors using enzymatic digestion as previously described . Briefly, the adipose tissue was extensively washed with two volumes of Hank’s Balanced Salt Solution (HBSS) containing 5% antibiotic/antimycotic solution (10,000 units of penicillin, 10,000 μg of streptomycin, and 25 μg of Amphotericin B per mL; HyClone), fragmented, and then digested at 37°C for 1 h in the presence of collagenase (200 U/ml, Sigma-Aldrich) and dispase (10 U/ml, BD Biosciences). Enzymatic activity was neutralized by adding an equal volume of culture medium (HyClone™ AdvanceSTEM™ Mesenchymal Stem Cell Basal Medium for human undifferentiated mesenchymal stem cells containing 10% of HyClone™ AdvanceSTEM™ Mesenchymal Stem Cell Growth Supplement (CGS), 1% antibiotic/antimycotic solution (HyClone) and centrifuged at 200 g for 10 min. This led to the sedimentation of diverse cells, including MSCs, macrophages, lymphocytes, and erythrocytes, unlike adipocytes that remained floating. After removal of supernatant, a lysis solution (154 mM NH4Cl, 10 mM KHCO3, and 0.1 mM EDTA) was added to a cell pellet to lyse erythrocytes, and cell suspension was centrifuged at 200 g for 10 min. Sedimented cells were resuspended in the MSC culture medium and filtered through a 100-μm nylon cell strainer (BD Biosciences). As indicated by flow , after isolation and overnight preplating, the obtained cell population contained not only MSC cells that basically represented the most abundant subgroup but also admixed macrophages and lymphocytes. The two last cell subgroups were dramatically depleted by culturing for a week in the MSC culture medium and humidified atmosphere (5% CO2) at 37°C. The obtained MSC population was maintained at a subconfluent level (~80% confluency) and passaged using HyQTase (HyClone). By using the methodology described previously , cultured cells were demonstrated to differentiate into the osteogenic, chondrogenic, and adipogenic directions, the finding confirming their multipotency. In experiments, MSCs of the second to fourth passages were usually used.
2.2. Preparation of cells for Ca2+ imaging
Before assaying with Ca2+ imaging, cells were maintained in a 12-socket plate for 12 h in the medium described above but without antibiotics. For isolation, cells cultured in a 1-ml socket were rinsed twice with the Versene solution (Sigma-Aldrich) that was then substituted for 200 μl HyQTase solution (HyClone) for 3–5 min. The enzymatic treatment was terminated by the addition of a 0.8 ml culture medium to a socket. Next, cells were resuspended, put into a tube, and centrifuged at 50 g for 45 s for moderate sedimentation. Isolated cells were collected by a plastic pipette and plated onto a photometric chamber of nearly 150 μl volume. The last was a disposable coverslip (Menzel-Glaser) with attached ellipsoidal resin wall. The chamber bottom was coated with Cell-Tak (BD Biosciences), enabling strong cell adhesion. Attached cells were then loaded with dyes for 20 min at room temperature (23–25°С) by adding Fluo-4 AM (4 μM) and Pluronic (0.02%; all from Molecular Probes) to a bath solution. Loaded cells were rinsed with the bath solution for several times and kept at 4°C for 1 h prior to recordings. Generally, incubation of MSCs at low temperature stabilized intracellular Ca2+ and decreased a fraction of spontaneously oscillating cells.
2.3. Ca2+ imaging and uncaging
Experiments were carried out using an inverted fluorescent microscope Axiovert 135 equipped with an objective Plan NeoFluar 20x/0.75 (Zeiss) and a digital EMCCD camera LucaR (Andor Technology). Apart from a transparent light illuminator, the microscope was equipped with a handmade system for epi-illumination via an objective. The epi-illumination was performed using a bifurcational glass fiber. One channel was used for Fluo-4 excitation and transmitted irradiation of a computer-controllable light-emitting diode (LED) LZ1-00B700H (LED Engin). LED emission was filtered with an optical filter ET480/20x (Chroma Technology). Fluo-4 emission was collected at 535 ± 25 nm by using an emission filter ET535/50 m (Chroma Technology). Serial fluorescent images were usually captured every second and analyzed using Imaging Workbench 6 software (INDEC). Within the 1-s acquisition period, the 480 nm LED was switched on for only 200 ms, during which cell fluorescence was collected. This protocol allowed for minimizing photobleaching of Fluo-4 at a sufficiently high signal-to-noise ratio achievable by adjusting LED emission. This enabled us to reliably assay cell responsiveness to different compounds applied serially for up to 60 min. Deviations of cytosolic Ca2+ from the resting level were quantified by a relative change in the intensity of Fluo-4 fluorescence (ΔF/F0) recorded from an individual cell.
Another channel was connected to a pulsed solid laser TECH-351 Advanced (680 mW) (Laser-Export, Moscow). This unit operated in a two harmonic mode and generated not only 351 nM UV light used for Ca2+ uncaging but also visible light at 527 nm. The last could penetrate into an emission channel through nonideal optical filters and elicit optical artifacts during uncaging. For Ca2+ or IP3 uncaging, cells were loaded with 4 μM Fluo-4-AM (Invitrogen) and 4 μM NP-EGTA-AM (Invitrogen) or 4 μM caged-Ins(145)P3/PM (SiChem) + 0.02% Pluronic (Invitrogen) for 30 min at 23°С. The basic bath solution contained (mM): 110 NaCl, 5.5 KCl, 2 CaCl2, 0.8 MgSO4, 10 glucose, 10 HEPES-NaOH, and pH 7.4 (≈270 Osm). When necessary, 2 mM CaCl2 in the bath was replaced with 0.5 mМ EGTA + 0.4 mМ CaCl2, thus reducing free Ca2+ to nearly 260 nM at 23°С as calculated with the Maxchelator program (http://maxchelator.stanford.edu). In this low Ca2+ bath solution, the glucose concentration was increased to 13 mM to keep osmolarity. All chemicals used in experiments described below were applied by the complete replacement of the bath solution in a 150-μl photometric chamber for nearly 2 s using a perfusion system driven by gravity. The used salts and buffers were from Sigma-Aldrich, and agonists and inhibitors were from Tocris.
In a typical experiment, nearly a hundred of MSCs loaded with Fluo-4 resided in a photometric camera, and their responsiveness to different ligands was assayed with Ca2+ imaging. Consistently with observations of others , functional heterogeneity was characteristic of a MSC population derived from each particular donor. Although a variety of GPCR agonists were found to stimulate Ca2+ signaling in MSCs, including ATP, ADP, noradrenaline or adrenaline, acetylcholine or its analog carbachol, GABA, glutamate, serotonin, and UTP, only a relatively small group of cells in a given MSC population was specifically responsive to a particular agonist (Figure 1). Overall, nearly 103 MSCs were sequentially stimulated by multiple agonists applied at different combinations, and a particular cell was either irresponsive to all stimuli or responded to one, rarely two, particular compound (Figure 1A–C). ATP-sensitive cells composed the most abundant subgroup of 9–15% (12% on average), depending on MSC preparation (Figure 1B). The percentage of cells responsive to other agonists was on average: ADP—7.1, adenosine—8.7, carbachol—3.4, GABA—5, glutamate—1.2, noradrenaline—6.7, serotonin—6.6, and UTP—6 (Figure 1B). The more or less accurate analysis of distribution of MSC responsivity was performed for nucleotides. In designated experiments, wherein cells were sequentially stimulated by ATP, ADP, and UTP, 125 purinergic MSCs were assayed overall, and only 13 cells (10%) were found to respond to all three agonists at the indicated concentrations (Figure 1C). Both ATP and ADP stimulated Ca2+ signaling in 40 cells (32%) that did not respond to UTP; 33 cells (26%) preferred the ATP-UTP pair. In addition, 20, 9, and 7 cells (16, 7, and 6%) responded exclusively to ATP, ADP, or UTP, respectively (Figure 1C).
Thus, the results presented above (Figure 1) clearly demonstrated that responsiveness to a given agonist varied from cell to cell. Note that GPCRs from most subfamilies, e.g. P2Y receptors, can couple to several signaling pathways, depending on cellular context [26, 27, 28, 29]. Hence, in cells nonresponsive in terms of Ca2+ signaling to a particular agonist, appropriate GPCRs might be either not expressed or not coupled to Ca2+ mobilization.
3.1. Dose dependence of MSC responses to adrenergic and purinergic agonists
In the present study, we focused on transduction of adrenergic and purinergic agonists capable of stimulating Ca2+ signaling in the MSC cytoplasm. We first aimed at evaluating dose dependencies of cellular responses to tested agonists. The analysis, which initially involved adrenergic transduction, revealed that Ca2+ responses varied with noradrenaline concentration in an “all-or-nothing” fashion. In other words, noradrenaline never caused detectable effects, when applied below 100 nM, but above the threshold of 100–200 nM, it elicited marked Ca2+ transients that were similarly shaped irrespective of agonist concentration (Figure 2A). Since we expected to obtain a somewhat gradual dose dependence, we considered the possibility that at concentrations used, noradrenaline might elicit too high Ca2+ transients, which all saturated Fluo-4 fluorescence, thus appearing alike. However, the permeabilizing agent saponin (0.1 mg/mL) evoked marked Ca2+ signals that exceeded noradrenaline responses by the factor of 1.5–2 (17 cells; Figure 2A). These observations indicated conclusively that MSC responses to varied noradrenaline could not be equalized due to saturation of the Ca2+ dye. The further analysis of MSC responsivity pointed out that the “all-or-nothing” phenomenon was intrinsic for the agonist-dependent Ca2+ signaling in general, including purinergic transduction. In particular, submicromolar ATP was ineffective, while the nucleotide elicited Ca2+ transients in the MSC cytoplasm at 1–2 μM and higher (Figure 2B). The adenosine responses were characterized by the threshold of 0.2–0.3 μM and were similarly shaped at higher concentrations (9 cells; Figure 2C). For ADP- and UTP-responses, the threshold concentrations ranged within 0.5–2 and 3–6 μM, respectively. Although we did not carefully characterize MSC responses to adenosine, ADP, and UTP at widely and gradually varied concentrations, it appeared that dose-response curves for these agonists were also step-like. For example, Ca2+ transients of close magnitudes were usually elicited by adenosine at 0.5 and 5 μM (21 cells), ADP at 1 and 30 μM (16 cells), and UTP at 3 and 50 μM (11 cells) (Figure 2C–F).
In the case of noradrenaline and ATP, the dose dependence of MSC responses was carefully evaluated in designated experiments, wherein an agonist dose was gradually varied in a wide range of concentrations (Figure 2A, B). During this prolonged assay, responsiveness of many cells was liable to rundown, thus impeding the quantitative analysis. Overall, we identified 21 cells that generated sufficiently robust responses to noradrenaline at 30 nM–10 μM with the threshold of 100–200 nM. Among them, 10 cells, which exhibited the same threshold of 150 nM, were taken for the analysis. To compare different experiments, responses of each particular cell recorded at variable agonist concentrations were normalized to a response to 1 μM noradrenaline and superimposed as shown in Figure 2G, where different symbols correspond to individual cells. Despite some data scattering, normalized cellular responses were localized in the narrow range of 0.8–1.2 (Figure 2G), clearly demonstrating that in all cases, the dose dependence was a step-like rather than gradual. Similar inference came from the analysis of 32 ATP-sensitive cells that showed quite robust responses to the nucleotide gradually applied at 0.5–50 μM. Of them, nine MSCs generated rather similar Ca2+ signals at gradually increasing ATP doses with the threshold of 1 μM (Figure 2B, H).
One more notable feature of MSC responses was that Ca2+ transients were markedly postponed relative to a moment of agonist application. The characteristic time of response delay (τd, Figure 3A) gradually decreased with noradrenaline and ATP concentration (Figure 3B, C). For instance, Ca2+ transients triggered by noradrenaline were retarded by 38–55 s at the threshold stimulation (Figure 3A, left response), whereas the delay was reduced to 17–26 s at the concentration of 1 μM and higher (Figure 3A, right response). The detailed assay of the dose-delay dependence was not carried out for the other agonists. Nevertheless, the comparison of MSCs responses obtained at low and saturated concentrations of adenosine, ADP, or UTP revealed a marked decrease in response delay as the agonist dose raised (Figure 3D). As discussed below, two distinct mechanisms are presumably responsible for specific dependencies of the magnitude and delay of MSC responses on agonist concentration.
3.2. Agonist transduction involves the phosphoinositide cascade and Ca2+-induced Ca2+ release
In certain experiments, we analyzed coupling of adreno- and purinoreceptors to Ca2+ mobilization in the MSC cytoplasm. When MSCs were pretreated with U73122 (2–5 μM), a poorly reversible inhibitor of PLC, all assayed cells became completely nonresponsive to tested agonists, including noradrenaline (17 cells), ATP (39 cells), adenosine (11 cells), UTP (7 cells), and ADP (5 cells) (Figure 4A–C, G–I). The inhibitory effect of U73122 on MSC responsiveness was apparently specific as the much less effective analog U73343 (2–5 μM) never canceled MSC responses to the nucleotides (Figure 4A–C, G, H). Moreover, the decrease of external Ca2+ from 2 mM to 260 nM weakly or negligibly affected Ca2+ transients elicited by ATP (26 cells), noradrenaline (31 cells), adenosine (7 cells), UTP (14 cells), and ADP (13 cells) (Figure 4C, D, G–I). Thus, the agonist-stimulated Ca2+ signaling in MSCs involved GPCRs that were basically coupled by the phosphoinositide cascade to Ca2+ release rather than to Ca2+ entry. Note also that the step-like dose dependence of ATP responses (Figure 2B, H) and their insignificant sensitivity to external Ca2+ (Figure 4G) indicated that P2X receptors could provide only a weak, if any, contribution to Ca2+ signaling triggered by ATP in the MSC cytoplasm.
Given the aforementioned effects of U73122 on MSC responses, there might be little doubt that the IP3 receptor, a common effector downstream of PLC , was involved in transduction of assayed agonist. Expectedly, the IP3 receptor blocker 2-APB (50 μM) suppressed Ca2+ signaling initiated by ATP (21 cells), noradrenaline (19 cells), adenosine (5 cells), ADP (9 cells), and UTP (10 cells) (Figure 4D–I)). In contrast, 50 μM ryanodine, a ryanodine receptor antagonist, was ineffective in all cases (Figure 4F–I). These findings suggested a negligible role for ryanodine receptors in agonist transduction. Consistently, their agonist caffeine (10 mM) insignificantly affected cytosolic Ca2+ in ATP-responsive MSCs (7 cells; Figure 4F). It should be noted that 2-APB blocks not only IP3 receptors but also a variety of Ca2+-entry channels [31, 32, 33]. Given however that MSC responsiveness to P2Y agonists insignificantly depended on external Ca2+ and therefore on Ca2+ influx (Figure 4G–I), we inferred that 2-APB exerted the inhibitory action mainly by targeting IP3 receptors.
The monotonic and gradual dependence of cellular responses on agonist concentration has been reported for a variety of cellular systems, including those that employ GPCRs coupling to Ca2+ mobilization [34, 35, 36]. In contrast, Ca2+ responses were generated by MSCs in an “all-or-nothing” manner (Figure 2). This step-like dose dependence of response magnitude is poorly explicable and apparently inconsistent with the gradual relation between response delay and agonist concentration (Figure 3) if agonist transduction involves solely PLC-dependent production of an IP3 burst and proportional Ca2+ release via IP3 receptors. To address this problem, we assumed that the agonist transduction occurred in two separated consecutive steps. Initially, an agonist produced a Ca2+ signal most likely being small, local, and gradually dependent on stimulus intensity. When exceeding the threshold, this local and poorly resolved Ca2+ signal pushed massive Ca2+-induced Ca2+ release (CICR) [37, 38, 39, 40] to accomplish transduction with a large and global Ca2+ signal. By involving the trigger-like mechanism CICR, a cell generates Ca2+ responses of virtually universal shape and magnitude at different agonist concentrations above the threshold (Figure 2). Rising with agonist proportionally, the initial gradual Ca2+ signal reached a CICR threshold for the time that should have shortened with agonist concentration, thus underlying the gradual dose-delay dependence observed (Figure 3B, C).
To clarify functionality of the CICR mechanism in MSCs and its contribution to agonist responses, we used Ca2+ uncaging that allowed for generating as fast and intensive cytosolic Ca2+ bursts as necessary for initiating the CICR process. In designated experiments, MSCs were loaded with both Fluo-4 and NP-EGTA. The last is photolabile Ca2+ chelator with high affinity to Са2+ (Kd ~ 10−7 М), so that in a resting cell (~100 nm free Са2+), nearly half NP-EGTA molecules are bound to Са2+ ions. The absorption of ultraviolet (UV) light by NP-EGTA disrupts the coordination sphere responsible for Ca2+ binding, thus liberating Ca2+ions and producing a step-like increase in cytosolic Ca2+ . Because a UV laser we employed for uncaging was in fact a biharmonic light source emitting at 351 and 527 nm, a light stimulus caused an optical artifact that was seen as a marked overshoot in a recording trace of cell fluorescence acquired at 535 ± 25 nm.
In this series, caged Ca2+ was released by moderate UV pulses during several seconds to somehow simulate the suggested Ca2+ signal initially produced by agonists in the MSC cytoplasm. As illustrated in Figure 5A, light stimuli triggered in adrenergic MSCs (n = 33) two fundamentally different types of Ca2+ responses. The relatively short, 2-s in the given case, UV pulse produced an optical artifact that was followed by a small Ca2+ jump without evident delay (Figure 5A, left panel, response 1 and right panel, thick line). This Ca2+ signal exhibited exponential relaxation presumably mediated by Ca2+ pumps. The sequential 4-s and 6-s UV flashes elicited biphasic Ca2+ transients of nonproportional magnitudes (Figure 5A, left panel). Indeed, compared to a 2-s UV pulse, one could expect 4- and 6-s light stimuli to liberate nearly twice and three times more Ca2+ ions, respectively. Meanwhile, 4-, 6-, and 8-s flashes usually triggered the similar Ca2+ transients that exceeded a response to a 2-s pulse by an order of magnitude (Figure 5A, left panel). None of the known Ca2+-dependent mechanisms but CICR could amplify and shape an initial Ca2+ signal produced by NP-EGTA photolysis in such a way (Figure 5A, right panel, response 1 vs. response 2). In addition, the representative cell (Figure 5A, left panel) was insensitive to 50 nM noradrenaline but similarly responded to the agonist at 0.5 and 1 μM concentrations. Similar results were obtained with other eight MSCs that tolerated prolonged serial stimulation with both UV and noradrenaline. Note that biphasic cell responses to light and noradrenaline were quite similar by shape and magnitude (Figure 5A, right panel, thin line 2 and circled line 3). Interestingly, light responses exhibited the delay that shortened with UV pulse duration (Figure 5, left panel). Similar experiments were performed with purinergic MSCs (n = 23) and basically identical results were obtained (Figure 5B). These findings support the idea that the delay of agonist responses (Figure 3) could be determined by the initial gradual Ca2+ signal.
Similar to Ca2+ uncaging (Figure 5A), uncaging of IP3 produced agonist-like responses in purinergic (n = 14) and adrenergic (n = 6) MSCs (Figure 5C). It was therefore possible that Ca2+ uncaging could simulate agonist-like responses by stimulating Ca2+-dependent PLC [42, 43, 44], which quickly generated a sufficient IP3 burst, thereby enhancing activity of IP3 receptors and triggering CICR. To verify this possibility, several adrenergic (n = 12) and purinergic (n = 7) MSCs loaded with NP-EGTA were subjected to Ca2+ uncaging in the presence of U73122. Although this PLC inhibitor expectedly rendered MSCs nonresponsive to the agonists, the cells normally responded to UV flashes (Figure 5D, E). The ineffectiveness of U73122 (Figure 5D, E, H) provided strong evidence that PLC activation was not obligatory for generating light responses, thereby demonstrating that CICR initiated by UV flashes was directly stimulated by Ca2+ ions liberated from NP-EGTA.
Reportedly, ryanodine and inositol 1,4,5-trisphosphate (IP3) receptors, Ca2+-gated Ca2+ release channels operating in the endo/sarcoplasmic reticulum, are exclusively responsible for CICR in apparently all cells [39, 42, 44]. To evaluate a relative contribution of IP3 and ryanodine receptors to CICR in MSCs, we examined effects of their antagonists on Ca2+ signals associated with Ca2+ uncaging. While 50 μM ryanodine was ineffective, 50 μM 2-APB dramatically and reversibly changed a shape and magnitude of UV responses in adrenergic (n = 16) and purinergic (n = 11) MSCs (Figure 5F–H). In the presence of 50 μM ryanodine, Ca2+ uncaging elicited agonist-like biphasic Ca2+ responses that were delayed relative to stimulatory UV flashes (Figure 5F, G, 2nd responses). Thus, despite the inhibition of ryanodine receptors, Ca2+ uncaging was still capable of stimulating robust CICR in MSCs responsive to the agonists. With 50 μM 2-APB in the bath, a UV pulse entailed a brief Ca2+ jump that relaxed monotonically and was smaller by the factor 3–4 (Figure 5F, G, 3rd responses; Figure 5H). This indicated that Ca2+ uncaging failed to initiate CICR with inhibited IP3 receptors. Moreover, when 2-APB was removed to restore activity of IP3 receptors, a UV flash triggered a biphasic Ca2+ transient again (Figure 5F, G, 4th responses). These observations indicated that basically IP3 receptors were responsible for CICR in adrenergic and purinergic MSCs.
3.3. Adrenoreceptor subtypes involved in Ca2+ signaling
Nine human genes encode adrenoreceptors, including α1Α, α1Β, α1D, α2Α, α2Β, α2C, β1, β2, and β3 isoforms . Previously, we demonstrated that transcripts for α1Β-, α2Α-, and β2-adrenoreceptors were invariably present in total MSC preparations . Given that both α1- and α2-adrenoreceptors are routinely coupled to PLC and Ca2+ mobilization in different cells [21, 22], either or both of these isoforms might be responsible for Ca2+ transients generated by MSCs in response to noradrenaline (Figure 2A). In contrast, β2-adrenoreceptors, which generally involve adenylyl cyclase as a downstream effector , could not be an essential contributor to Ca2+ signaling in adrenergic MSCs.
To uncover a role of the particular isoform, we performed recordings using agonists and antagonists specific for α1- or α2-adrenoreceptors. Overall, 35 noradrenaline-responsive cells were treated with phenylephrine/cirazoline and prazosin (α1-agonists and antagonist, respectively) as well as with guanabenz/B-HT 933 and yohimbine (α2-agonists and antagonist, respectively). Most of them (29 cells, 83%) were irresponsive to phenylephrine (1–10 μM), and their noradrenaline responses were not inhibited by 10 μM prazosin. In contrast, guanabenz (10–50 μM) and B-HT 933 (10 μM) were quite effective (Figure 6A). In particular, 50 μM guanabenz stimulated Ca2+ signaling in all noradrenaline-responsive MSCs (Figure 6A–C). Consistently, 2 μM yohimbine dumped cellular responses to noradrenaline and guanabenz (Figure 6A). Six cells (17%) were sensitive to both 10 μM phenylephrine and 50 μM guanabenz (Figure 6B, C). These findings indicate that the α2-subtype, evidently α2Α, predominantly mediates Ca2+ signaling initiated by noradrenaline in MSCs, although in a minor MSC subpopulation, both α1- and α2-isoforms could be involved in adrenergic transduction.
3.4. Effects of isoform-specific agonists and antagonists of P2Y receptors
In mammalians, the P2Y subgroup includes eight GPCRs (P2Y1,2,4,6,11–14) that exhibit certain specificities to nucleotides, depending on species [18, 46]. The expression of purinoreceptors in MSCs was analyzed previously, and transcripts for multiple P2Y receptors were detected, namely, P2Y1, P2Y2, P2Y4, P2Y6, P2Y11, P2Y13, and P2Y14, while P2Y12 transcripts were not detected in total MSC preparations . Although this P2Y array is sufficient to account for MSC capability to detect ATP, ADP, and UTP, it was impossible to evaluate a contribution of a particular P2Y isoform based on MSC responses to these natural P2Y agonists (Figure 2B, E, F). To address this issue, we used isoform-specific P2Y agonists and antagonists.
The human P2Y family contains two ATP receptors, including specialized P2Y11 and also P2Y2 that recognizes both UTP and ATP as full equipotent agonists . Although also known as a partial P2Y1 agonist, ATP was hardly capable of stimulating P2Y1-signaling in MSCs at low micromolar concentrations due to much lower efficacy than ADP . We tried to evaluate a contribution of P2Y11 and P2Y2 to MSC responsiveness to ATP. Among 181 MSCs assayed in this series, 169 cells (93%) became nonresponsive to ATP (3 μM) in the presence of 30 μM NF 340, a specific P2Y11 antagonist. These NF 340-sensitive cells did not respond to the P2Y2agonist MRS 2768 (10 μM) (Figure 7A, cell 1 and Figure 7B). In a subpopulation of rare MSCs (12 cells) that were capable of generating Ca2+ transients on 3 μM ATP in the presence of NF 340, 11 cells also responded to 10 μM MRS 2768 (Figure 7A, cell 2 and Figure 7B). Thus, MSCs that were insensitive to NF 340 presumably employed P2Y2 or both P2Y2 and P2Y11 to detect ATP.
While the P2Y11 antagonist was highly effective (Figure 7A, B), most ATP-sensitive MSCs were surprisingly nonresponsive to NF 546 (10 μM), the specific P2Y11 agonist reported to be even more effective than ATP . Among 127 cells that responded to 3 μM ATP, 10 μM NF 546 stimulated Ca2+ signaling solely in 9 cells (7%; Figure 7C, D). At the moment, we cannot provide any valid explanation for very low efficacy of NF-546 relative to ATP (Figure 7D). Perhaps, this synthetic ligand is a biased agonist that enables coupling of P2Y11 to the phosphoinositide cascade by involving only a certain G-protein type, which is absent or relatively less abundant in most of the MSCs.
UTP is a full agonist for P2Y2 and P2Y4 that were identified in MSCs at the population level . It therefore was unclear whether a particular cell employs either or both of these P2Y receptors for monitoring extracellular UTP. We analyzed the sensitivity of 95 UTP-responsive MSCs to MRS 2768 and MRS 4062, specific agonists of P2Y2 and P2Y4 receptors, respectively. Consistently with the analysis of ATP-responsive cells (Figure 7B), we found only 9 (9.5%) of 95 UTP-sensitive cells to react to 10 μM MRS 2768 (Figure 8A, cell 3 and Figure 8B). In contrast, 78 cells (82%) responded to 10 μM MRS 4062 (Figure 7A, cell 1 and Figure 7B). These findings suggested that predominantly P2Y4 was responsible for Ca2+ signaling evoked in MSCs by UTP, while P2Y2 was either expressed in a very small subpopulation of P2Y4-negative cells or not coupled to Ca2+ mobilization in a great majority of P2Y4-positive cells.
Extracellular ADP is detected by cells with P2Y1, P2Y12, and P2Y13. The analysis of ADP responsiveness was performed on 102 MSCs sensitive to 3 μM ADP (Figure 8A) that might be recognized by P2Y1 and/or P2Y13 receptors, given that P2Y12 transcripts were not found in MSCs. To evaluate a role of the P2Y1, 65 of 103 ADP-sensitive MSCs were treated with MRS 2365, a highly potent and selective P2Y1 agonist that displays no activity at P2Y12 and P2Y13 at submicromolar concentrations . MRS 2365 was ineffective at 100–300 nM but triggered Ca2+ signaling in 16 (25%) of 65 MSCs at 10 μM (Figure 9A). Because MRS 2365 specifically stimulates P2Y1 with EC50 ~ 1 nM , this agonist might bring about a nonspecific action at 10 μM. On the other hand, MRS 2179 (10 μM), a P2Y1 antagonist with IC50 = 0.15 μM , inhibited ADP responses in all MRS 2365-treated MSCs (65 cells; Figure 9A). Given that other P2Y receptors were hardly inhibited by 10 μM MRS 2179 , the observed effects of the specific agonist and antagonist of the P2Y1 receptor were rather inconsistent. To reconcile these contradictory findings, we considered the possibility that both P2Y1 and P2Y13 should have been activated by ADP concurrently to mobilize Ca2+ in MSCs. If so, nanomolar MRS 2365 was ineffective, activating solely P2Y1, while 10 μM MRS 2365 stimulated activity of both P2Y1 and P2Y13 , thus triggering Ca2+ signaling in MSCs. This concept predicted that MSCs would be unable to respond to ADP if either P2Y1 or P2Y13 was inhibited. In line with this idea, we assayed sensitivity of 51 ADP-responsive MSCs to both MRS 2179 (10 μM) and MRS 2211 (10 μM), a P2Y13 antagonist. It turned out that either of these compounds rendered each of 51 assayed cells nonresponsive to ADP (Figure 9B, C). Altogether, our findings (Figure 9A–C) indicated that only those MSCs, which functionally expressed both P2Y1 and P2Y13 receptors, were capable of generating robust Ca2+ responses to ADP.
Virtually in all cell types, extracellular cues can mobilize intracellular Ca2+ to regulate a variety of diverse cellular functions, such as fertilization, proliferation, secretion, metabolism, gene expression, mobility, and muscle contraction. How can the Ca2+ ion, a chemically simple substance, control so many different physiological processes? The plausible explanation comes from the versatility of Ca2+ signaling mechanisms that can mediate Ca2+ signals with variable kinetics, amplitude, duration, and spatial patterning, depending on cellular context and stimulation [30, 37, 42].
Transduction of multiple agonists involves GPCRs coupled to PLCβ1–4 isoforms that hydrolyze the precursor lipid phosphatidylinositol 4,5-bisphosphate to produce two second messengers, IP3 and diacylglycerol. The primary mode of action of IP3 is to bind to IP3 receptors and release Ca2+ from the endoplasmic reticulum (ER) [30, 51, 52]. Three different isoforms of the IP3 receptor have been identified (IP3R1, IP3R2, and IP3R3) and shown to serve as a tetrameric IP3-gated Ca2+ channel [30, 51, 52, 53]. IP3R1, IP3R2, and IP3R3 are distinct by physiological properties, thus allowing cells to generate specific Ca2+ signals with different spatial and temporal characteristics to control diverse cellular functions [30, 52]. In addition to IP3, Ca2+ is the primary coregulator of IP3 receptors [30, 51, 52, 54]. The full activation of the IP3 receptor occurs when IP3 has occupied the IP3-binding domains on all four subunits . This is associated with a conformational change, which sensitizes the Ca2+-binding site. The binding of cytosolic Ca2+ to this site markedly increases the open probability of the IP3 receptor channel , so that Ca2+ ions released from the ER can additionally stimulate activity of IP3 receptors. This positive feedback mediates CICR. Meanwhile, the action of cytosolic Ca2+ is bimodal: stimulating IP3 receptors at low levels, Ca2+ becomes inhibitory above 300 nm . This multimodal control of the IP3 receptor by IP3 and Ca2+ is central to various aspects of intracellular Ca2+ signaling [30, 52].
In the present work, we studied MSCs from the human adipose tissue and examined intracellular Ca2+ signaling initiated by certain GPCR agonists, including adenosine, ATP, noradrenaline, and some others. Although all first messengers tested here were effective, only a relatively small MSC group responded to a particular agonist. These specifically responsive cell subpopulations overlapped weakly or negligibly, depending on agonists (Figure 1). This finding is hardly surprising in light of a widely accepted idea that a MSC population from different sources represents a heterogeneous mixture of diverse cells, including multipotent and more committed progenitor cells [1, 3, 56, 57]. Yet, cultured MSCs are not synchronized and dwell in different phases of the cell cycle. It therefore might be expected that divergent intracellular signaling is inherent in a MSC population containing both proliferating and quiescent cells. The aforementioned factors could underlie intrinsic heterogeneity of a MSC population discussed previously [56, 57]. It also should be mentioned that most of assayed MSCs were found by us nonresponsive to a particular agonist solely in terms of Ca2+ signaling that necessitated coupling of appropriate GPCRs to Ca2+ mobilization. Meanwhile, many GPCR isoforms are in fact promiscuous in that they may be coupled to a variety of downstream signaling pathways, depending on G-proteins involved. For instance, the P2Y1,2,4,6,11 subtypes of purinoreceptors are canonically coupled by Gq/G11 to the phosphoinositide cascade and Ca2+ mobilization, whereas P2Y12,13,14 control cAMP production by inhibiting adenylyl cyclase through Gi/Go. The unique capability of P2Y11 is to stimulate Gs . In addition, apart from ubiquitous coupling to PLC and adenylyl cyclase, P2Y receptors can also engage effectors such as MAP, PI3, Akt, and PKC kinases; small G-proteins; NO synthase; transactivation of growth factor receptors; and some others [26, 27, 28, 29]. Hence, a fraction of MSCs sensitive to a given agonist might be in fact much more abundant than that evaluated by Ca2+ imaging (Figure 1B, C), because the tested compounds could stimulate not only Ca2+ mobilization but also other signaling events.
The agonist-dependent Ca2+ signaling in MSCs was mostly detailed by us for noradrenaline and certain nucleotides. By using subtype-specific agonists and antagonists, it was shown that mainly a2-adrenoreceptors mediated Ca2+ mobilization triggered by noradrenaline in adrenergic MSCs (Figure 6). In purinergic MSCs, presumably P2Y11 serves as a primary ATP receptor (Figure 7), UTP responsiveness is largely mediated by P2Y4 (Figure 8), while both P2Y1 and P2Y13 are involved in detecting ADP (Figure 9). The responsivity of MSCs to noradrenaline and ATP and apparently to adenosine, ADP, and UTP exhibited a peculiar dose dependence: undetectably affecting intracellular Ca2+ below the cut-off concentration, a particular agonist initiated Ca2+ transients that were large and quite similarly shaped at all doses above the threshold (Figure 2). In contrast to this step-like dose-response curve, the dependence of response delay on agonist concentration was gradual (Figure 3). The inhibitory analysis and Ca2+ uncaging approach showed that agonist transduction universally involved the classical phosphoinositide cascade and CICR mechanism (Figures 4 and 5) that employed IP3 receptors rather than ryanodine receptors (Figures 4E, F and 5F, G).
To reconcile the “all-or-nothing” dose-response curve and gradual dose-delay dependence, we surmised that agonist-evoked Ca2+ signaling in MSCs includes two different but coupled stages. Primarily, agonists stimulate IP3 production, activation of IP3 receptors, and generation of an initial, presumably local and gradual Ca2+ signal. Next, this local Ca2+ signal stimulates CICR that produces a global Ca2+ signal. Some evidence suggests that the Ca2+ store responsible for the initial Ca2+ signal may be physically separated from the Ca2+ store that provides CICR. Indeed, when cells were overloaded with NP-EGTA due to the twofold excess of NP-EGTA-AM concentration compared to the standard loading protocol (see Methods), a MSC population became poorly sensitive to ATP. However, several UV flashes usually rendered MSC responsive (Figure 10). Presumably, overloading with NP-EGTA excessively increased the Ca2+-buffering capacity of the cell cytoplasm, thereby significantly diminishing the initial agonist-induced Ca2+ signal and its speed. The photodistraction of NP-EGTA decreased exogenous Ca2+ buffer to a physiologically more relevant level, thus recovering MSC responsiveness to ATP. Note that in line with multiple reports, relatively slow Ca2+ buffer EGTA is unable to cancel Ca2+-dependent processes mediated by local intracellular Ca2+ signals. For instance, 1 mM EGTA does not prevent activation of Ca2+-gated BK channels by Ca2+ transients originated by both Ca2+ influx via voltage-gated Ca2+ channels and Ca2+ release stimulated by muscarine . By analogy and based on the observation that Ca2+ uncaging was still capable of triggering CICR in MSCs overloaded with NP-EGTA (Figure 10), we suggested that NP-EGTA, slow Ca2+ buffer , could hardly repeal stimulation of IP3 receptors by Ca2+ ions released through this IP3-gated conduit. If so, the Ca2+ store and IP3 receptor pool mediating CICR should be spatially separated from agonist-dependent machinery that generates an initial, local, and gradual Ca2+ signal. Otherwise, it is difficult to explain why in cells overloaded with NP-EGTA, agonist responses disappeared contrary to light responses associated with Ca2+ uncaging (Figure 10).
Note in conclusion that the specific features of agonist responses, including kinetics and magnitude, all-or-nothing behavior and gradual dose-response delay were correctly reproduced by Ca2+ signals elicited by Ca2+ uncaging (Figure 5). This supports the idea that agonist-evoked Ca2+ signaling in MSCs includes two different but coupled stages. Initially, agonists stimulate coupling of suitable GPCRs via appropriate G-proteins to PLC, thus triggering IP3 production, activation of IP3 receptors (IP3Rgrad) followed by the release of Ca2+ ions from Ca2+ store. This machinery generates an initial, presumably local and gradual Ca2+ signal (Figure 11). When exceeding the threshold, this local Ca2+ signal stimulates CICR that is mediated by IP3 receptors (IP3RCICR) presumably located in another, spatially separated Ca2+ store. By involving the trigger-like mechanism CICR, a cell generates Ca2+ responses of virtually universal shape and magnitude at different agonist concentrations above the cut-off dose. Of course, the presented model is a simplification of the actual transduction process, and roles for other common contributors to intracellular Ca2+ signaling, including Ca2+ pumps, mitochondria, Ca2+ buffer as well as Ca2+-dependent enzymes and ion channels, remain to be elucidated.
We thank Dr. V. Yu. Sysoeva for providing MSCs of the first passage. We are thankful to the Russian Science Foundation for support of studies of adrenergic and purinergic transduction (grant 18-14-0034) and P2Y receptors (grant 17-75-10127).
Kalinina NI, Sysoeva VY, Rubina KA, Parfenova YV, Tkachuk VA. Mesenchymal stem cells in tissue growth and repair. Acta Naturae. 2011; 3:30-37
Keating A. Mesenchymal stromal cells: New directions. Cell Stem Cell. 2012; 10:709-716. DOI: 10.1016/j.stem.2012.05.015
Baer PC. Adipose-derived mesenchymal stromal/stem cells: An update on their phenotype in vivo and in vitro. World journal of stem cells. 2014; 6:256-265. DOI: 10.4252/wjsc.v6.i3.256
Nordberg RC, Loboa EG. Our fat future: Translating adipose stem cell therapy. Stem Cells Translational Medicine. 2015; 4:974-979. DOI: 10.5966/sctm.2015-0071
Casiraghi F, Perico N, Cortinovis M, Remuzzi G. Mesenchymal stromal cells in renal transplantation: Opportunities and challenges. Nature Reviews. Nephrology. 2016; 12:241-253. DOI: 10.1038/nrneph.2016.7
Lou G, Chen Z, Zheng M, Liu Y. Mesenchymal stem cell-derived exosomes as a new therapeutic strategy for liver diseases. Experimental & Molecular Medicine. 2017; 49:e346. DOI: 10.1038/emm.2017.63
Scarfi S. Purinergic receptors and nucleotide processing ectoenzymes: Their roles in regulating mesenchymal stem cell functions. World Journal of Stem Cells. 2014; 6:153-162. DOI: 10.4252/wjsc.v6.i2.153
Forostyak O, Forostyak S, Kortus S, Sykova E, Verkhratsky A, Dayanithi G. Physiology of Ca2+ signalling in stem cells of different origins and differentiation stages. Cell Calcium. 2016; 59:57-66. DOI: 10.1016/j.ceca.2016.02.001
Penicaud L. Relationships between adipose tissues and brain: What do we learn from animal studies? Diabetes and Metabolism. 2010; 36:S39-S44. DOI: 10.1016/S1262-3636(10)70465-1
Cavaliere F, Donno C, D'Ambrosi N. Purinergic signaling: A common pathway for neural and mesenchymal stem cell maintenance and differentiation. Frontiers in Cellular Neuroscience. 2015; 9:211. DOI: 10.3389/fncel.2015.00211
Glaser T, Cappellari AR, Pillat MM, Iser IC, Wink MR, Battastini AM, Ulrich H. Pers-pectives of purinergic signaling in stem cell differentiation and tissue regeneration. Purinergic Signal. 2012; 8:523-537. DOI: 10.1007/s11302-011-9282-3
Jiang LH, Hao Y, Mousawi F, Peng H, Yang X. Expression of P2 purinergic receptors in mesenchymal stem cells and their roles in extracellular nucleotide regulation of cell functions. Journal of Cellular Physiology. 2017; 232:287-297. DOI: 10.1002/jcp.25484
Ciciarello M, Zini R, Rossi L, Salvestrini V, Ferrari D, Manfredini R, Lemoli RM. Extra-cellular purines promote the differentiation of human bone marrow-derived mesenchymal stem cells to the osteogenic and adipogenic lineages. Stem Cells and Development. 2013; 22:1097-1111. DOI: 10.1089/scd.2012.0432
Gharibi B, Abraham AA, Ham J, Evans BA. Contrasting effects of A1 and A2b adenosine receptors on adipogenesis. International Journal of Obesity. 2012; 36:397-406. DOI: 10.1038/ijo.2011.129
Zimmermann H, Zebisch M, Strater N. Cellular function and molecular structure of ecto-nucleotidases. Purinergic Signal. 2012; 8:437-502. DOI: 10.1007/s11302-012-9309-4
Fredholm BB, IJzerman AP, Jacobson KA, Linden J, Muller CE. International Union of Basic and Clinical Pharmacology. LXXXI. Nomenclature and classification of adenosine receptors – An update. Pharmacological Reviews. 2011; 63:1-34. DOI: 10.1124/pr.110.003285
Fields RD, Burnstock G. Purinergic signalling in neuron-glia interactions. Nature Reviews Neuroscience. 2006; 7:423-436. DOI: 10.1038/nrn1928
Burnstock G. Purinergic signalling: From discovery to current developments. Experi-mental Physiology. 2014; 99:16-34. DOI: 10.1113/expphysiol.2013.071951
Saul A, Hausmann R, Kless A, Nicke A. Heteromeric assembly of P2X subunits. Frontiers in Cellular Neuroscience. 2013; 7:250. DOI: 10.3389/fncel.2013.00250
Samways DS, Li Z, Egan TM. Principles and properties of ion flow in P2X receptors. Frontiers in Cellular Neuroscience. 2014; 8:6. DOI: 10.3389/fncel.2014.00006
Cotecchia S. The α1-adrenergic receptors: Diversity of signaling networks and regulation. Journal of Receptor and Signal Transduction Research. 2010; 30:410-419. DOI: 10.3109/10799893.2010.518152
Cottingham C, Chen H, Chen Y, Peng Y, Wang Q. Genetic variations of a2-adrenergic receptors illuminate the diversity of receptor functions. Current Topics in Membranes. 2011; 67:161-190. DOI: 10.1016/B978-0-12-384921-2.00008-2
Lynch GS, Ryall JG. Role of beta-adrenoceptor signaling in skeletal muscle: Implications for muscle wasting and disease. Physiological Reviews. 2008; 88:729-767. DOI: 10.1152/physrev.00028.2007
Kotova PD, Sysoeva VY, Rogachevskaja OA, Bystrova MF, Kolesnikova AS, Tyurin-Kuzmin PA, Fadeeva JI, Tkachuk VA, Kolesnikov SS. Functional expression of adrenoreceptors in mesenchymal stromal cells derived from the human adipose tissue. Biochimica et Biophysica Acta. 2014; 1843:1899-1908. DOI: 10.1016/j.bbamcr.2014.05.002
Kalinina N, Kharlampieva D, Loguinova M, Butenko I, Pobeguts O, Efimenko A, Ageeva L, Sharonov G, Ischenko D, Alekseev D, Grigorieva O, Sysoeva V, Rubina K, Lazarev V, Govorun V. Characterization of secretomes provides evidence for adipose-derived mesenchymal stromal cells subtypes. Stem Cell Research & Therapy. 2015; 6:221. DOI: 10.1186/s13287-015-0209-8
Buvinic S, Briones R, Huidobro-Toro JP. P2Y1 and P2Y2 receptors are coupled to the NO/cGMP pathway to vasodilate the rat arterial mesenteric bed. British Journal of Pharmacology. 2002; 136:847-856. DOI: 10.1038/sj.bjp.0704789
Montiel M, de la Blanca EP, Jimenez E. P2Y receptors activate MAPK/ERK through a pathway involving PI3K/PDK1/PKC-zeta in human vein endothelial cells. Cellular Physiology and Biochemistry: International Journal of Experimental Cellular Physiology, Biochemistry and Pharmacology. 2006; 18:123-134. DOI: 10.1159/000095180
Luke TM, Hexum TD. UTP and ATP increase extracellular signal-regulated kinase 1/2 phosphorylation in bovine chromaffin cells through epidermal growth factor receptor transactivation. Purinergic Signal. 2008; 4:323-330. DOI: 10.1007/s11302-008-9098-y
Malaval C, Laffargue M, Barbaras R, Rolland C, Peres C, Champagne E, Perret B, Terce F, Collet X, Martinez LO. RhoA/ROCK I signalling downstream of the P2Y13 ADP-receptor controls HDL endocytosis in human hepatocytes. Cellular Signaling. 2009; 21:120-127. DOI: 10.1016/j.cellsig.2008.09.016
Berridge MJ. The inositol trisphosphate/calcium signaling pathway in health and disease. Physiological Reviews. 2016; 96:1261-1296. DOI: 10.1152/physrev.00006.2016
Xu SZ, Zeng F, Boulay G, Grimm C, Harteneck C, Beech DJ. Block of TRPC5 channels by 2-aminoethoxydiphenyl borate: A differential, extracellular and voltage-dependent effect. British Journal of Pharmacology. 2005; 145:405-414. DOI: 10.1038/sj.bjp.0706197
Mustafa T, Walsh J, Grimaldi M, Eiden LE. PAC1hop receptor activation facilitates catecholamine secretion selectively through 2-APB-sensitive Ca2+ channels in PC12 cells. Cellular Signaling. 2010; 22:1420-1426. DOI: 10.1016/j.cellsig.2010.05.005
Harteneck C, Gollasch M. Pharmacological modulation of diacylglycerol-sensitive TRPC3/6/7 channels. Current Pharmaceutical Biotechnology. 2011; 12:35-41. DOI: 10.2174/138920111793937943
Berg KA, Clarke WP, Sailstad C, Saltzman A, Maayani S. Signal transduction differences between 5-hydroxytryptamine type 2A and type 2C receptor systems. Molecular Pharmacology. 1994; 46:477-484
Baryshnikov SG, Rogachevskaja OA, Kolesnikov SS. Calcium signaling mediated by P2Y receptors in mouse taste cells. Journal of Neurophysiology. 2003; 90:3283-3294. DOI: 10.1152/jn.00312.2003
Petrel C, Kessler A, Dauban P, Dodd RH, Rognan D, Ruat M. Positive and negative allosteric modulators of the Ca2+-sensing receptor interact within overlapping but not identical binding sites in the transmembrane domain. The Journal of Biological Chemistry. 2004; 279:18990-18997. DOI: 10.1074/jbc.M400724200
Berridge MJ, Bootman MD, Roderick HL. Calcium signaling: Dynamics, homeostasis and remodeling. Nature Reviews. Molecular Cell Biology. 2003; 4:517-529. DOI: 10.1038/nrm1155
Clapham DE. Calcium Signaling. Cell. 2007; 131:1047-1058. DOI: 10.1016/j.cell.2007.11.028
Iino M. Spatiotemporal dynamics of Ca2+ signaling and its physiological roles. Proceedings of the Japan Academy. Series B, Physical and Biological Sciences. 2010; 86:244-256
Thomas NL, Williams AJ. Pharmacology of ryanodine receptors and Ca2+-induced Ca2+ release. Wiley Interdisciplinary Reviews: Membrane Transport and Signaling. 2012; 1:383-397. DOI: 10.1002/wmts.34
Ellis-Davies GC. Caged compounds: Photorelease technology for control of cellular chemistry and physiology. Nature Methods. 2007; 4:619-628. DOI: 10.1038/nmeth1072
Dupont G, Combettes L, Leybaert L. Calcium dynamics: Spatio-temporal organization from the subcellular to the organ level. International Review of Cytology. 2007; 261:193-245. DOI: 10.1016/S0074-7696(07)61005-5
Park JB, Lee CS, Jang JH, Ghim J, Kim YJ, You S, Hwang D, Suh P-G, Ryu SH. Phospholipase signalling networks in cancer. Nature Reviews. Cancer. 2012; 12:782-792. DOI: 10.1038/nrc3379
Kawamoto EM, Vivar C, Camandola S. Physiology and pathology of calcium signaling in the brain. Frontiers in Pharmacology. 2012; 3:61. DOI: 10.3389/fphar.2012.00061
Guimaraes S, Moura D. Vascular adrenoceptors: An update. Pharmacological Reviews. 2001; 2:319-356
Verkhratsky A, Burnstock G. Biology of purinergic signalling: Its ancient evolutionary roots, its omnipresence and its multiple functional significance. BioEssays: News and Reviews in Molecular, Cellular and Developmental Biology. 2014; 36:697-705. DOI: 10.1002/bies.201400024
Kotova PD, Bystrova MF, Rogachevskaja OA, Khokhlov AA, Sysoeva VY, Tkachuk VA, Kolesnikov SS. Coupling of P2Y receptors to Ca2+ mobilization in mesenchymal stromal cells from the human adipose tissue. Cell Calcium. 2018; 71:1-14. DOI: 10.1016/j.ceca.2017.11.001
Waldo GL, Harden TK. Agonist binding and Gq-stimulating activities of the purified human P2Y1 receptor. Molecular Pharmacology. 2004; 65:426-436. DOI: 10.1124/mol.65.2.426
von Kugelgen I, Hoffmann K. Pharmacology and structure of P2Y receptors. Neuro-pharmacology. 2016; 104:50-61. DOI: 10.1016/j.neuropharm.2015.10.030
Chhatriwala M, Ravi RG, Patel RI, Boyer JL, Jacobson KA, Harden TK. Induction of novel agonist selectivity for the ADP-activated P2Y1 receptor versus the ADP-activated P2Y12 and P2Y13 receptors by conformational constraint of an ADP analog. The Journal of Pharmacology and Experimental Therapeutics. 2004; 311:1038-1043. DOI: 10.1124/jpet.104.068650
Foskett JK, White C, Cheung KH, Mak DO. Inositol trisphosphate receptor Ca2+ release channels. Physiological Reviews. 2007; 87:593-658. DOI: 10.1152/physrev.00035.2006
Mikoshiba K. Role of IP3 receptor signaling in cell functions and diseases. Advances in Biological Regulation. 2015; 57:217-227. DOI: 10.1016/j.jbior.2014.10.001
Taylor CW, da Fonseca PCA, Morris EP. IP3 receptors: The search for structure. Trends in Biochemical Science. 2004; 29:210-219. DOI: 10.1016/j.tibs.2004.02.010
Mak DO, Foskett JK. Inositol 1,4,5-trisphosphate receptors in the endoplasmic reticulum: A single-channel point of view. Cell Calcium. 2015; 58:67-78. DOI: 10.1016/j.ceca.2014.12.008
Alzayady KJ, Wang L, Chandrasekhar R, Wagner LE 2nd, Van Petegem F, Yule DI. Defining the stoichiometry of inositol 1,4,5-trisphosphate binding required to initiate Ca2+ release. Science Signaling. 2016; 9:ra35. DOI: 10.1126/scisignal.aad6281
Phinney DG. Functional heterogeneity of mesenchymal stem cells: Implications for cell therapy. Journal of Cellular Biochemistry. 2012; 113:2806-2812. DOI: 10.1002/jcb.24166
Galle J, Hoffmann M, Krinner A. Mesenchymal stem cell heterogeneity and ageing in vitro: A model approach. In: Geris L, editor. Computational Modeling in Tissue Engineering. Berlin, Heidelberg: Springer Berlin Heidelberg; 2013. pp. 183-205. DOI: 10.1007/8415_2012_116
Prakriya M, Solaro CR, Lingl CJ. [Ca2+]i elevations detected by BK channels during Ca2+ influx and muscarine-mediated release of Ca2+ from intracellular stores in rat chromaffin cells. Journal of Neuroscience. 1996; 16:4344-4359. DOI: 10.1523/JNEUROSCI.16-14-04344.1996
Faas GC, Karacs K, Vergara JL, Mody I. Kinetic properties of DM-Nitrophen binding to calcium and magnesium. Biophysical Journal. 2005; 88:4421-4433. DOI: 10.1529/biophysj.104.057745