Heterotrimeric G-protein subunit Gαi2 contributes to agonist-sensitive apoptosis and degranulation in murine platelets.

Gαi2 , a heterotrimeric G-protein subunit, regulates various cell functions including ion channel activity, cell differentiation, proliferation and apoptosis. Platelet-expressed Gαi2 is decisive for the extent of tissue injury following ischemia/reperfusion. However, it is not known whether Gαi2 plays a role in the regulation of platelet apoptosis, which is characterized by caspase activation, cell shrinkage and cell membrane scrambling with phosphatidylserine (PS) translocation to the platelet surface. Stimulators of platelet apoptosis include thrombin and collagen-related peptide (CoRP), which are further known to enhance degranulation and activation of αIIb β3-integrin and caspases. Using FACS analysis, we examined the impact of agonist treatment on activation and apoptosis in platelets drawn from mice lacking Gαi2 and their wild-type (WT) littermates. As a result, treatment with either thrombin (0.01 U/mL) or CoRP (2 μg/mL or 5 μg/mL) significantly upregulated PS-exposure and significantly decreased forward scatter, reflecting cell size, in both genotypes. Exposure to CoRP triggered a significant increase in active caspase 3, ceramide formation, surface P-selectin, and αIIb β3-integrin activation. These molecular alterations were significantly less pronounced in Gαi2 -deficient platelets as compared to WT platelets. In conclusion, our data highlight a previously unreported role of Gαi2 signaling in governing platelet activation and apoptosis.

Introduction

Heterotrimeric G proteins are coupled to plasma membrane receptors and participate in the regulation of a wide range of cellular functions such as migration, differentiation, proliferation, ion channel activity, and apoptosis (Hilger et al. 2018; Squires et al. 2018). In platelets, fundamental elements of the hemostasis machinery, a wide array of cell surface receptors coupled to G proteins mediate their activation (Offermanns 2006). The P2Y12 receptor, an important therapeutic target contributing to purinergic stimulation of platelets, is coupled to heterotrimeric Gα i2 protein, the predominant Gα isoform (Gachet 2012). More recently, Gα i2 protein was reported to play a thrombo‐inflammatory role in orchestrating thrombus stabilization during hemostasis and mediating tissue damage during experimental cerebral and myocardial ischemia‐reperfusion injury (Devanathan et al. 2015).

Platelets are activated by a wide range of agonists such as subendothelial collagen, thrombin, ADP secreted from stimulated platelets, and by collagen‐related peptide (CoRP) (Lang et al. 2013). In the presence of stimulatory signals, platelets degranulate, undergo phospholipid scrambling on their cell membrane, and aggregate to form thrombi that results in vascular blockage (Varga‐Szabo et al. 2009; Munzer et al. 2014). Cell membrane scrambling with phosphatidylserine (PS) exposure fosters the assembly of tenase and prothrombinase complexes, and subsequently promoting factor Xa and thrombin generation (Lebois and Josefsson 2016). In platelets, unconstrained apoptosis has been implicated in thrombocytopenia, bleeding disorders, microparticle shedding as well as affecting their quality during storage (Lebois and Josefsson 2016; Quach et al. 2018). PS exposure in apoptotic platelets, triggered by exogenous agents or physiological changes, leads to their clearance from the circulation (Lebois and Josefsson 2016; Quach et al. 2018). Gα i2 has previously been shown to participate in the apoptosis machinery of different cell types (Lopez‐Aranda et al. 2008; Bissinger et al. 2016). Despite the recent evidence linking Gα i2 protein to the execution of thrombosis, its role in platelet survival has hitherto remained elusive. In the present study, using thrombin and collagen‐related peptide (CoRP), an agonist mimicking the effect of contact with collagen and a powerful stimulator of platelet apoptosis (Munzer et al. 2018), we investigated the influence of Gα i2 on platelet survival and degranulation ex vivo.

Materials and Methods

Mice

Experiments were performed in Gα i2‐deficient mice (Gα ) and their wild‐type (WT) littermates of 10–12 weeks of age. The mice were generated and initially characterized on a SV129 background (Rudolph et al. 1995). Mice were backcrossed on a C57BL/6 background and kept under specified pathogen‐free (SPF) environment in individually ventilated cages (IVC) to prolong life expectancy (Wiege et al. 2013; Devanathan et al. 2015). All animal experiments were conducted according to the German law for the care and use of laboratory animals and were approved by local government authorities (Regierungspräsidium Tübingen according to §4 of 19/12/2011).

Preparation of mouse platelets

Platelets were obtained from 10‐ to 12‐week‐old mice of either sex which were treated according to the protocol approved by government authorities. Eight hundred μl blood was obtained into tubes containing 200 μl acid‐citrate‐dextrose buffer. Platelet rich plasma (PRP) was obtained by centrifugation at 260 g for 5 min. PRP was then centrifuged at 640 g for 5 min to pellet the platelets. Where necessary, apyrase (0.02 U/mL; Sigma‐Aldrich) and prostaglandin I2 (0.5 μmol/L; Calbiochem) were added to the PRP to prevent activation of platelets during isolation. After two washing steps, the pellet of washed platelets was resuspended in modified Tyrode‐HEPES buffer (pH 7.4, supplemented with 1 mmol/L CaCl2). Where indicated, thrombin (0.01 U/mL, Roche, Basel, Switzerland) or collagen‐related peptide (CoRP, 2 μg/mL or 5 μg/mL, kindly provided by R. Farndale, University of Cambridge, Cambridge, UK) were added (Liu et al. 2016).

Cytosolic calcium

For the measurement of the cytosolic Ca2+ concentration, the platelet preparation was washed once in Tyrode buffer (pH 7.4), stained with 3 μmol/L Fluo‐3AM (Biotium, USA) in the same buffer and incubated at 37°C for 30 min. Following the indicated experimental treatment, relative fluorescence was measured utilizing a BD FACS Calibur (BD Biosciences, Heidelberg, Germany) (Towhid et al. 2011; Liu et al. 2016).

P‐selectin and activated integrin abundance

Fluorophore‐labeled antibodies were utilized for the detection of P‐selectin expression (Wug.E9‐FITC, Emfret Analytics, Eibelstadt, Germany) and the active form of α IIb β3 integrin (JON/A‐PE, Emfret Analytics, Eibelstadt, Germany). Washed mouse platelets (1x106) were suspended in modified Tyrode buffer (pH 7.4) containing 1 mmol/L CaCl2 and antibodies (1:10 dilution) and subsequently subjected to the respective treatments and for the indicated time periods at room temperature (RT). The reaction was stopped by addition of PBS and the samples were immediately analyzed by FACS analysis (Liu et al. 2015).

Phosphatidylserine exposure and forward scatter

Phosphatidylserine exposure was determined in platelets with and without a 10 min thrombin or CoRP treatment (Liu et al. 2016). To this end, the platelet preparation was centrifuged at 660 g for 5 min followed by washing once with Tyrode buffer (pH 7.4) with 1 mmol/L CaCl2, staining with 1:20 dilution of Annexin‐V FITC (ImmunoTools, Germany) in Tyrode buffer (pH 7.4) in the presence of 2 mmol/L CaCl2 and incubation at 37°C for 30 min. Annexin‐V binding reflecting surface exposure of phosphatidylserine was evaluated by FACS analysis. In parallel, the forward scatter (FSC) of the platelets was determined by FACS analysis, as a measure of platelet size (Liu et al. 2016).

Caspase‐3 activity

Caspase 3 activity was determined utilizing a CaspGlow Fluorescein Active Caspase‐3 Staining kit from BioVision (CA, USA) according to the manufacturer's instruction. Fluorescence intensity was measured at an excitation wavelength of 488 nm and an emission wavelength of 530 by FACS analysis.

Ceramide abundance

Ceramide abundance at platelet cell surface was measured by a monoclonal antibody‐assay. For this purpose, platelets were stained at 37°C for 1 h at a concentration of 1 μg/mL anti‐ceramide antibody (clone MID 15B4, Enzo Life Science GmbH, Lörrach, Germany) in Tyrode buffer at a dilution of 1:10. Platelets were washed once with Tyrode buffer. Subsequently, platelets were stained for 30 min with polyclonal fluorescein isothiocyanate (FITC) conjugated goat anti‐mouse IgG and IgM specific antibody (BD Pharmingen, Hamburg, Germany) at a concentration of 1:50 in Tyrode buffer. Washing of the platelets was performed in order to remove unbound secondary antibody. Finally, the samples were analyzed by flow cytometry at an excitation wavelength of 488 nm and an emission wavelength of 530 nm, as has previously been shown (Gatidis et al. 2010).

Statistical analysis

Data are shown as means ± SD; n represents the number of independent experiments. All data were tested for significance using ANOVA. P < 0.05 was considered statistically significant.

Results

This study addressed the impact of Gα i2 on activation and apoptosis of murine platelets. For this purpose, experiments were performed in mice lacking Gα i2 and corresponding wild type mice. The platelets were analyzed with or without prior exposure to thrombin (0.01 U/mL) or collagen‐related peptide (CoRP, 2 μg/mL and 5 μg/mL). Individual values (mean ± SD) of female and male WT and Gα i2‐deficient mice of annexin‐V‐binding, platelet volume, caspase‐3‐positive cells, ceramide abundance, P‐selectin abundance and activated integrin α IIb β3 are displayed in Table 1A–D. No significant differences were observed between male and female WT or Gα i2‐deficient mice.

Table 1

Analyzed parameters in WT and Gα i2‐deficient mice

A: Annexin‐V‐binding and forward scatter in WT female and male mice
Parameter	WT (female)			WT (male)
	Resting	Thrombin	CoRP	Resting	Thrombin	CoRP
Annexin‐V‐binding [%]	0.89 ± 0.02	17.07 ± 2.50	19.22 ± 0.87	1.06 ± 0.39	18.22 ± 2.34	18.60 ± 2.75
Forward Scatter [Geomean; arb. units]	14.95 ± 1.00	10.43 ± 0.95	8.15 ± 0.18	15.09 ± 0.46	11.29 ± 1.03	9.42 ± 1.11

Annexin‐V‐binding, forward scatter, P‐selectin abundance, activated integrin α IIb β3, caspase‐3‐positive cells, and ceramide abundance in female and male WT and Gα i2‐deficient mice after thrombin and/or CoRP stimulation.

Phosphatidylserine exposure, a hallmark of platelet apoptosis, was quantified by flow cytometry analysis using annexin‐V‐binding as described previously (Cao et al. 2017). As illustrated in Figure 1A and D, the percentage of PS‐positive platelets in untreated resting Gα and WT platelets was not significantly different. Treatment with thrombin and CoRP significantly enhanced the percentage of PS‐positive platelets, an effect significantly less pronounced in Gα platelets as compared to WT platelets (Fig. 1B–D). Next, we explored whether Gα i2‐mediated platelet apoptosis accompanies cell volume alterations (Cao et al. 2017). As depicted in Figure 1E and H, forward scatter, reflecting platelet volume, was not significantly different in resting platelets of either genotype but was significantly reduced following thrombin and CoRP treatment, an effect significantly less pronounced in Gα platelets than in WT platelets (Fig. 1F–H).

Figure 1

Gαi2 participates in the regulation of platelet cell membrane scrambling and platelet volume. (A–C) Original histogram overlays of the annexin‐V binding in platelets isolated from WT mice (blue shadow) and Gα i2‐deficient mice (black line) without (A) and with (B) a 10 min treatment with thrombin (0.01 U/mL) or (C) a 10 min treatment with collagen‐related peptide CoRP (5 μg/mL). (D) Arithmetic means ± SD (n = 4) of the annexin‐V binding in platelets isolated from WT mice (blue bar) and Gα i2‐deficient mice (black bar) prior to (control) and following a 10 min treatment with thrombin (0.01 U/mL) or a 10 min treatment with collagen‐related peptide CoRP (5 μg/mL). ### (P < 0.001) indicates statistically significant difference from absence of thrombin and CoRP, * (P < 0.05) and *** (P < 0.001) indicates statistically significant difference from WT mice. (E–G) Original histogram overlays of the forward scatter of platelets isolated from WT mice (blue shadow) and Gα i2‐deficient mice (black line) without (E) and with (F) a 10 min treatment with thrombin (0.01 U/mL) or (G) a 10 min treatment with collagen‐related peptide CoRP (5 μg/mL). (H) Arithmetic means ± SD (n = 4) of the forward scatter of platelets isolated from WT mice (blue bar) and Gα i2‐deficient mice (black bar) prior to (control) and following a 10 min treatment with thrombin (0.01 U/mL) or a 10 min treatment with collagen‐related peptide CoRP (5 μg/mL). ### (P < 0.001) indicates statistically significant difference from absence of thrombin and CoRP, * (P < 0.05) and *** (P < 0.001) indicates statistically significant difference from WT mice.

We then sought to elucidate the mechanism(s) regulating Gα i2‐mediated apoptosis. To this end, we analyzed intracellular Ca2+ levels [Ca2+]i in murine platelets of either genotype using Fluo3 AM fluorescence as described previously (Cao et al. 2017). As a result, prior to CoRP treatment, [Ca2+]i in resting platelets was similar in Gα platelets (22.73 ± 0.69, a.u.; n = 10) and in WT platelets (20.95 ± 0.50, a.u.; n = 10). Treatment with CoRP was followed by a profound and significant increase of [Ca2+]i in both Gα (109.3 ± 1.46, a.u., n = 10) and WT platelets (105.9 ± 0.69, a.u.; n = 10). The increase following CoRP treatment was, however, not significantly different between the two genotypes, thus, ruling out the involvement of Ca2+ signaling in Gα i2‐mediated platelet apoptosis.

Next, we explored whether other putative mechanisms underpin the regulation of Gα i2‐mediated platelet apoptosis. To this end, caspase 3 fluorescence (Cao et al. 2017) was measured and was similar in resting platelets of either genotype (Fig. 2A and C), but was significantly upregulated after CoRP treatment, an effect which was significantly blunted in Gα platelets as compared to WT platelets (Fig. 2B and C).

Figure 2

Gαi2 participates in the regulation of platelet caspase 3 activation and ceramide formation. (A and B) Original histogram overlays of the caspase 3 activity in platelets isolated from WT mice (blue shadow) and Gα i2‐deficient mice (black line) without (A) and with (B) a 10 min treatment with collagen‐related peptide CoRP (5 μg/mL). (C) Arithmetic means ± SD (n = 6) of the caspase 3 activity (arbitrary units) in platelets isolated from WT mice (blue bar) and Gα i2‐deficient mice (black bar) prior to (control) and following a 10 min treatment with collagen‐related peptide CoRP (5 μg/mL). ### (P < 0.001) indicates statistically significant difference from absence of CoRP, *** (P < 0.001) indicates statistically significant difference from WT mice. (D and E) Original histogram overlays of the ceramide abundance of platelets isolated from WT mice (blue shadow) and Gα i2‐deficient mice (black line) without (D) and with (E) a 10 min treatment with collagen‐related peptide CoRP (5 μg/mL). (F) Arithmetic means ± SD (n = 4) of the ceramide abundance of platelets isolated from WT mice (blue bar) and Gα i2‐deficient mice (black bar) prior to (control) and following a 10 min treatment with collagen‐related peptide CoRP (5 μg/mL). ## (P < 0.01) indicates statistically significant difference from absence of CoRP, ** (P < 0.01) indicates statistically significant difference from WT mice.

As has previously been shown, hyperosmotic shock triggered a significant increase in platelet annexin‐V‐binding, an effect probably involving ceramide formation (Gatidis et al. 2010). We thus examined whether ceramide formation is altered in Gα i2‐deficient platelets as compared to WT platelets. As illustrated in Figure 2D and F, ceramide abundance was similar in resting platelets. CoRP treatment elicited a significant increase in ceramide abundance in WT platelets as compared to Gα platelets (Fig. 2E and F), pointing to the involvement of sphingomyelinase activation in the triggering of Gα i2‐mediated platelet apoptosis.

We then tested whether Gα i2 similarly mediates platelet degranulation in response to CoRP. To this end, P‐selectin expression was similar in untreated resting and Gα platelets (Fig. 3A and C). Exposure to CoRP significantly increased P‐selectin expression (Cao et al. 2017) on the platelet surface reflecting enhanced degranulation; this effect was significantly reduced in Gα platelets as compared to WT platelets (Fig. 3B and C). Next, we explored whether active integrin α IIb β3 is different in the two genotypes. As a result, active integrin α IIb β3 was similar in WT and Gα platelets (Fig. 3D and F). In addition, CoRP treatment further stimulated active integrin α IIb β3 (Cao et al. 2017) at the platelet surface, an effect that was again significantly attenuated in Gα platelets (Fig. 3E and F). Thus, Gα i2 is dichotomously involved in both platelet degranulation and apoptosis following agonist exposure.

Figure 3

Gαi2 participates in the regulation of platelet degranulation and integrin α b β3 activation. (A and B) Original histogram overlays of P‐selectin‐related fluorescence reflecting degranulation in platelets isolated from WT mice (blue shadow) and Gα i2‐deficient mice (black line) without (A) and with (B) a 15 min treatment with collagen‐related peptide CoRP (2 μg/mL). (C) Arithmetic means ± SD (n = 6) of the P‐selectin‐related fluorescence (arbitrary units) in platelets isolated from WT mice (blue bar) and Gα i2‐deficient mice (black bar) prior to (control) and following a 15 min treatment with collagen‐related peptide CoRP (2 μg/mL). ### (P < 0.001) indicates statistically significant difference from absence of CoRP, * (P < 0.05) indicates statistically significant difference from WT mice. (D and E) Original histogram overlays of the α b β3 integrin‐related fluorescence in platelets isolated from WT mice (blue shadow) and Gα i2‐deficient mice (black line) without (D) and with (E) a 15 min treatment with collagen‐related peptide CoRP (2 μg/mL). (F) Arithmetic means ± SD (n = 6) of the α b β3 integrin‐related fluorescence (arbitrary units) in platelets isolated from WT mice (blue bar) and Gα i2‐deficient mice (black bar) prior to (control) and following a 15 min treatment with collagen‐related peptide CoRP (2 μg/mL). ### (P < 0.001) indicates statistically significant difference from absence of CoRP, *** (P < 0.001) indicates statistically significant difference from WT mice.

Discussion

Previous studies have shown that the effect of CoRP on degranulation, PS exposure, cell volume, and α IIb β3 integrin abundance is mediated, at least in part, by increased [Ca2+]i (Varga‐Szabo et al. 2009; Lang et al. 2013), which is known to trigger platelet activation and stimulate arterial thrombosis (Lang et al. 2013). Surprisingly, elevation of [Ca2+]i was similar in platelets of either genotype suggesting that Gα i2 modifies platelet activation and apoptosis by interfering with mechanisms other than Ca2+ entry.

Acid sphingomyelinase degrades membrane sphingomyelin and generates ceramide, which is responsible for cell membrane scrambling and degranulation in a variety of cell types; this lipid signaling is vital in the pathophysiology of several cardiovascular diseases (Lang et al. 2015). Remarkably, both genetic deficiency and pharmacological inhibition of acid sphingomyelinase has been shown to thwart platelet secretion and PS exposure independently of Ca2+ signaling, purportedly due to a signaling defect downstream of phospholipase C activation (Munzer et al. 2014). Ceramide metabolism further involves ceramidases which has been reported to ameliorate CoRP‐triggered glycoprotein VI‐dependent platelet aggregation and thrombus formation (Munzer et al. 2018). Along these lines, it is tempting to speculate that PS‐exposure and degranulation of platelets mediated by Gα i2‐sensitive ceramide generation is a possible mechanism linking previous observations of tissue injury and thrombosis after experimental ischemia‐reperfusion.

In conclusion, the present study sheds light on a novel function of Gα i2 protein, that is, the regulation of platelet apoptosis, a process, at least in part, mediated by agonist‐sensitive ceramide formation. Our observations on Gα i2‐mediated platelet survival may have pathophysiological implications in thrombo‐inflammatory conditions. Further investigations are warranted to dissect the relevance of this mechanism in platelet‐related disorders in humans.

Conflict of Interest

The authors state that they have no conflict of interest.