Piperlongumine Blocks JAK2-STAT3 to Inhibit Collagen-Induced Platelet Reactivity Independent of Reactive Oxygen Species†

Hengjie Yuan; Katie L. Houck; Ye Tian; Uddalak Bharadwaj; Ken Hull; Zhou Zhou; Mingzhao Zhou; Xiaoping Wu; David J. Tweardy; Daniel Romo; Xiaoyun Fu; Yanjun Zhang; Jianning Zhang; Jing-fei Dong

doi:10.1371/journal.pone.0143964

Abstract

Background

Piperlongumine (PL) is a compound isolated from the piper longum plant. It possesses anti-cancer activities through blocking the transcription factor STAT3 and by inducing reactive oxygen species (ROS) in cancer, but not normal cells. It also inhibits platelet aggregation induced by collagen, but the underlying mechanism is not known.

Objective

We conducted in vitro experiments to test the hypothesis that PL regulates a non-transcriptional activity of STAT3 to specifically reduce the reactivity of human platelets to collagen.

Results

PL dose-dependently blocked collagen-induced platelet aggregation, calcium influx, CD62p expression and thrombus formation on collagen with a maximal inhibition at 100 μM. It reduced platelet microvesiculation induced by collagen. PL blocked the activation of JAK2 and STAT3 in collagen-stimulated platelets. This inhibitory effect was significantly reduced in platelets pretreated with a STAT3 inhibitor. Although PL induced ROS production in platelets; quenching ROS using excessive reducing agents: 20 μM GSH and 0.5 mM L-Cysteine, did not block the inhibitory effects. The NADPH oxidase inhibitor Apocynin also had no effect.

Conclusions

PL inhibited collagen-induced platelet reactivity by targeting the JAK2-STAT3 pathway. We also provide experimental evidence that PL and collagen induce different oxidants that have differential effects on platelets. Studying these differential effects may uncover new mechanisms of regulating platelet functions by oxidants in redox signals.

Citation: Yuan H, Houck KL, Tian Y, Bharadwaj U, Hull K, Zhou Z, et al. (2015) Piperlongumine Blocks JAK2-STAT3 to Inhibit Collagen-Induced Platelet Reactivity Independent of Reactive Oxygen Species^†. PLoS ONE 10(12): e0143964. https://doi.org/10.1371/journal.pone.0143964

Editor: Zhenyu Li, University of Kentucky, UNITED STATES

Received: August 6, 2015; Accepted: November 11, 2015; Published: December 8, 2015

Copyright: © 2015 Yuan et al. This is an open access article distributed under the terms of the Creative Commons Attribution License, which permits unrestricted use, distribution, and reproduction in any medium, provided the original author and source are credited

Data Availability: All relevant data are within the paper and its Supporting Information files.

Funding: This work is supported by 1) grants HL71895 and HL085769 from the National Heart, Lung, and Blood Institute and CA149783 from the National Cancer Institute; 2) the Cancer Prevention and Research Institute of Texas (RP100421); 3) the Tianjin Science and Technology Support Program of China (No.14ZCZDSY00020); 4) the Natural Science Foundation of China (No.13JCYBJC21900 and 12JCYBJC31500); 5) the John S. Dunn Gulf Coast Consortium for Chemical Genomics Discovery Project; and 6) Tianjin Natural Science Foundation of China (No.13JCYBJC21900) and Tianjin Municipal Science and Technology Project (No.14ZCZDSY00020).

Competing interests: The authors have declared that no competing interests exist.

Introduction

The long pepper (Piper longum) is a member of the Piper genus known to possess anti-allergenic, anti-inflammatory, and liver protecting properties [1;2]. The fruit of P. longum has more than 600 known active compounds; among them is piperlongumine (PL, 5,6-dihydro-1-[1-oxo-3-(3,4,5-trimethoxyphenyl]-2(1H) pyridinone). PL, related compounds, and chemically synthesized analogs are reported to have anti-cancer [2;3], gastric protective [4], anti-microbial [5;6], adipogeneic [7;8], and anti-atherosclerotic activities [9]. PL executes these diverse activities, in part, by targeting protein synthesis at the transcriptional and post-transcriptional levels [3;10–12]. Raj L, et al [11] reported that PL selectively induces the death of cancer or transformed cells, while preserving the viability of normal cells in vitro and in vivo. This targeted activity relies on PL’s ability to increase intracellular reactive oxygen species (ROS), especially hydrogen peroxide and nitric oxide [11]. PL does so by binding and down-regulating activities of the enzymes glutathione S-transferase pi 1 (GSTP1) and carbonyl reductase 1 (CBR1)[11], resulting in a redox potential that is significantly tilted towards oxidation[3;11].

Paradoxically, PL was also reported to inhibit platelet activation, secretion, and aggregation induced by collagen, arachidonic acid, thromboxane, and platelet activating factor [13–15]. However, the known mechanisms involved in the inhibition of cancer cells do not support PL’s actions in platelets. First, blocking gene transcription is unlikely to play a significant role in the anti-platelet activity of PL because platelets are anucleated cells with a limited capacity for protein synthesis. Furthermore, the inhibitory effect was detected within minutes after PL treatment, insufficient for significant transcription and/or translation activities to occur. Second, ROS is known to activate platelets and promote thrombosis [16;17]. Cross-linking GP VI by collagen stimulates platelets to produce ROS [18]. These conflicting data lead to a critical question of whether PL induces these diverse phenotypic changes in platelets and cancer cells by targeting different molecules or by acting on a single molecule that is active both transcriptionally and non-transcriptionally. A target of PL specifically for collagen-induced platelet activation and aggregation that emerged from our recent study is the transcription factor STAT3 [19].

STAT3 is a member of a family of seven closely related proteins and serves as a key signaling protein in the IL-6-induced acute phase reaction pathway [20]. In nucleated cells, IL-6 binds to the IL-6Rα-gp130 receptor complex, oligomerizing receptors to activate receptor-associated tyrosine kinases. These activated kinases phosphorylate tyrosine residues to create a docking site for STAT3 via its Src-homology 2 (SH2) domain [21], leading to the phosphorylation of STAT3 at residue Y705 and the formation of a tail-to-tail homo-dimer that accumulates in the nucleus to regulate the transcription of targeted genes. We have recently uncovered a non-transcriptional role of STAT3 in a cross-talk between inflammatory IL-6-STAT3 and hemostatic/thrombotic collagen-GP VI signals that renders platelets hyper-reactive in conditions of inflammation through a trans-signaling mechanism [22].

These published reports have led us to hypothesize that PL regulates a non-transcriptional activity of STAT3 to reduce platelet reactivity to collagen. Here, we present data from in vitro experiments on human platelets using PL and synthesized derivatives to support this hypothesis. This study was not designed to study the pharmacokinetics of PL, but to identify PL’s molecular target(s) in regulating collagen-induced platelet activity and to explore roles of oxidative stress in platelet reactivity.

Materials and Methods

Reagents

Commercial reagents used in the study included: PL (Cayman Chemical Co., Ann Arbor, MI), the STAT3 inhibitor STA21 (Sigma Aldrich, St. Louis, MO), the JAK2-inhbitor AG490 (InvivoGen, San Diego, CA), the Syk inhibitor SykII (Merck Millipore, Billerica, MA), human recombinant IL-6 (R & D Systems, Minneapolis, MN), the extracellular domain of human IL-6 receptor-α (R & D Systems), Actinomycin (Sigma Aldrich), apocynin (Abcam Biochemicals. Cambridge, MA), free glutathione (GSH, Sigma Aldrich), L-cysteine (Sigma Aldrich), N-ethylmaleimide (NEM, Sigma Aldrich); dithiothreitol (DTT, Sigma Aldrich), fibrillary type I collagen (Helena laboratories, Beaumont, TX) and FITC-conjugated annexin V (BD Bioscience, San Jose, CA). Antibodies used in the study were: a FITC-conjugated monoclonal CD62p (BD Bioscience), a PE-conjugated monoclonal anti-CD42b (BD Bioscience), and antibodies for total and phosphorylated JAK2, STAT3, Syk, and PLCγγ2 (all from Cell Signaling Technologies, Danvers, MA).

Methods

Platelet aggregation.

Whole blood was collected (anticoagulant: 3.2% sodium citrate) from healthy donors under protocol #20121746 approved by the Western Institutional Review Board for Bloodworks Northwest via written informed consent. Platelet-rich plasma (PRP) was obtained by centrifugation of whole blood at 120 x g for 20 min at 26°C. Platelet counts in PRP were normalized to 3.0 x 10⁵ platelets/μl with homologous plasma and treated with PL (12.5–100 μM), its synthetic analogs or other testing agents for 15 min at 37°C. Platelet aggregation was induced in an optical aggregometer (Helena Laboratories) by fibrillar type I collagen or a collagen-related peptide (CRP) [22] and monitored for 5 min at 37°C. Collagen was tested primarily at 5 μg/ml in order to test the inhibitory strength of PL activity, which is recommended by the manufacturer for clinical tests, but also tested at 2 and 10 μg/ml in a subset of experiments in order to detect the effects of PL on different concentrations of collagen. PL was also tested for platelet aggregation induced by 5 μM of ADP or 50 μM of thrombin receptor activating peptide (TRAP). To identify the target of PL, the following reagents were tested either alone or in combination with PL at doses indicated in the result section: STA21, AG490, SykII, Actinomycin-D, Apocynin, GSH and L-Cysteine.

Platelet activation.

The effect of PL on collagen-induced platelet activation was measured by monitoring CD62p expression and calcium influx. CD62 expression was determined through the binding of a FITC-conjugated monoclonal antibody in PRP that was sequentially treated with PL and fibrillar type I collagen (0.5–10 μg/ml), each for 15 min at 37°C. For collagen-induced platelet calcium mobilization, 20 μl of PRP was mixed with 180 μl of Tyrode's buffer (138 mM NaCl, 2.9 mM KCl, 1.4 mM MgCl₂, 0.8 mM CaCl₂, 12 mM NaHCO₃, 5.5 mM glucose, pH 6.5) containing the Calcium Sensor Dye eFluor 514 (5 μM, final concentration, ebioscience, Inc., San Diego, CA). The mixture was immediately analyzed by flow cytometry [23]. Single platelets were gated on forward scatter and analyzed for fluorescence intensity over 60 sec to obtain the basal level. They were then stimulated with collagen, and monitored for changes in fluorescence intensity for additional 5 min at room temperature.

Hopping Probe Ion Conductance Microscopy imaging.

The effects of PL on the morphological changes and microvesiculation of platelets adherent to collagen were monitored using a modified ICnano Hopping Probe Ion Conductance Microscope (HPICM, Ionscope Ltd, UK) as previously described [24]. Briefly, PL-treated PRP was incubated on immobilized collagen (10 μg/ml, 4°C overnight) for 30 min at 37°C. After washing, adherent platelets were scanned under an ICnano scan head with a nanopipette (d = 60 nm) connected to an external Axon MultiClamp 700B amplifier (Molecular Devices, USA). This amplifier monitored the ion-current flowing into the nanopipette tip and supplied a DC voltage of +200 mV between the nanopipette electrode and bath electrode. All experiments were carried out at 24–28°C. Raw topography data were continuously acquired and linearly interpolated into images with ScanIC Image Viewer software version 1.0 (Ionscope Ltd, UK).

Measurement of platelet microparticles.

Platelet microvesiculation induced by collagen in the presence or absence of PL was detected by flow cytometry [24]. The supernatant from PRP placed on immobilized collagen (30 min at 37°C) was collected and centrifuged at 16,000x g to remove intact platelets. It was then incubated with a PE-conjugated CD42b antibody and FITC-conjugated annexin V for 20 min at room temperature; and fixed in a HEPES buffered saline containing 2.5 mM of CaCl₂ and 1% paraformaldehyde. MPs were first identified on particle size gated on forward scatter with a mixture of 0.5, 1.0 and 1.5 μm polystyrene standard beads (BD Bioscience) and then detected for CD42b expression and annexin V binding.

PL on thrombus formation.

Whole blood samples from healthy subjects were incubated with testing reagents for 20 min at 37°C. They were then perfused over immobilized collagen (coating density: 100 μg/ml, 4°C, overnight) at a flow rate that generated a shear stress of 60 dynes/cm² for 4 min at room temperature in an 8 channel microfluidic chamber (Cellix Mirus Nanopump^™, Dublin, Ireland). The chamber was then washed with PBS for additional 4 min. Images of thrombi formed on the collagen matrix were recorded at 400 x magnification under an Olympus IX-81 inverted stage microscope.

Immunoblots.

Washed platelets in Tyrode’s buffer were treated first with a testing agent and then with collagen or/and a mixture of recombinant human IL-6 and the extracellular domain of human IL-6 receptor-α (IL-6-sIL-6α). They were solubilized with a 10X hypotonic lysis buffer (120 mM Tris, 36 mM EDTA, and 10% Triton X-100, pH 7.5) in the presence of a cocktail of protease and phosphatase inhibitors (Sigma Aldrich). Platelet lysates were centrifuged at 13,000 x g for 15 min at 4°C to obtain the supernatant, which was separated on 4–12% gradient SDS polyacrylamide gel electrophoresis (PAGE) and probed for phosphorylated and total JAK2, STAT3, Syk, and PLCγ2 with specific antibodies.

Effect of PL on ROS production.

Three techniques were used to detect ROS production and its impact on PL activity in collagen treated platelets. First, intracellular ROS was measured by flow cytometry using a cell permeable dye DCFH-DA (Sigma Aldrich), which remains non-fluorescent until the acetate groups are removed by intracellular esterases upon oxidative stress. The dye probe primarily detects HO^., ONOO-, ROO^., and H₂O₂ species. PRP (150 μl) was diluted in 450 μl of Ca2⁺-free HEPES buffered Tyrode’s (138 mM NaCl, 5.5 mM glucose, 10 mM HEPES, 12 mM NaHCO₃, 2.9 mM KCl, 0.4 mM NaH₂PO₄, 0.4 mM MgCl₂, and 0.1% BSA, pH 7.2) and incubated with 10 μM of DCFH-DA (final concentration) for 30 min at 37°C. The dye-labeled platelets were analyzed after being treated with 100 μM of PL and/or 10 μg/ml of collagen for 20 min at 37°C. For data validation, the ROS probe CellROX (Life technologies, Grand Island, NY) that detects a similar set of oxidants as DCFH-DA was also tested.

Second, to measure free GSH in platelets, platelets in PRP were normalized to 250,000/μl with platelet-poor plasma and divided into 3 groups, each containing 7.5 x 10⁷ platelets. PRP in two groups were treated with either 100 μM of PL or 10 μg/ml of collagen (final concentrations) for 10 min without stirring. PRP in the third group was left untreated to set a baseline. The treated PRP was incubated with 10 mM of freshly prepared NEM for 60 min at 37°C to block free GSH on and in platelets. The NEM alkylated platelets were quickly frozen at -80°C, thawed on ice and sonicated using a Thermo Fisher Scientific Sonic Dismembrator. The homogenized samples were mixed with isotopically labeled GSH (Sigma Aldrich) internal standard. Proteins were precipitated with methanol and the supernatant was dried by Speed-Vac. Disulfide bonded GSH was reduced by 10mM DTT and newly released free GSH further alkylated by NEM. Total GSH was analyzed using liquid chromatography-tandem mass spectrometry with multiple reaction monitoring (LC-MS/MS-MRM) on an AB Sciex QTrap 6500 mass spectrometer coupled to a Waters Ultra Performance Liquid Chromatographer with Cortex C18 column. The percent of free GSH was calculated by dividing free GSH with total GSH.

Third, to examine a role of ROS production in PL-mediated inhibition, platelets were preincubated with either 20 μM of cell non-permeable GSH or 0.5 mM of cell permeable L-Cysteine for 15 min at 37°C to quench the intracellular and extracellular ROS before being sequentially treated with PL and collagen. The reduced nicotinamide adenine dinucleotide phosphate (NADPH) oxidase inhibitor Apocynin was also similarly tested.

PL derivatives.

All reactions were carried out under a nitrogen atmosphere in flame-dried glassware except for the hydrogenation reaction. Dichloromethane was purified by passage through activated alumina (solvent purification system). 1H and 13C NMR spectrum were recorded on INOVA-500. 1H NMR chemical shifts are reported as δ values in ppm relative to CDCl3 (7.26 ppm), coupling constants (J) are reported in Hertz (Hz), and multiplicity follows convention. Unless indicated otherwise, deuterochloroform (CDCl3) served as an internal standard (77.2 ppm) for all 13C spectra. Flash column chromatography was performed using 60Å Silica Gel (230–400 mesh) as a stationary phase using a gradient solvent system. Mass spectra were obtained at the center for Chemical Characterization and Analysis (Texas A&M University). Thin layer chromatography (TLC) was performed using silica gel 60 F254 coated glass-back TLC plates.

To generate compound 1 (C1), a mixture of piperlongumine (30 mg, 0.095 mmol) and 10 mg of Pd/C (10 wt.% Pd/C, 0.0094 mmol, 1% equiv) in 10 mL of EtOAc under H2 was stirred at 20°C for 2 h, then was filtered through to a short celite pad. The pad was washed with 10 ml of EtOAc. The solution was concentrated and the crude product was purified by a silica gel flash chromatography (Hexanes:EtOAc = 1:1) to give the desired product as a colorless oil (29 mg, 95%).

Compound 2 (C2) was prepared as a potential probe compound to aid in the identification of the biological target of PL and to provide structure-activity relationships (SAR). C2 has an alkyne group (a latent functional group for further derivatization) that can be used to add additional groups, such as biotin or a fluorophore) that can be used to identify the mode of action of PL. Selective cleavage of the methyl ether at the 4-position of the aromatic ring of PL was achieved using aluminum trichloride in dichloromethane at 0°C to give an intermediate compound in a high yield. Alkylation of the phenol with propargyl bromide produced the alkynyl derivative C2 in 67% yield. Hydrogenation of PL in ethyl acetate gave derivative compound 1 in 95% yield and provided an additional compound for SAR.

Statistical analyses.

Categorical (frequency) variables were expressed as percentages and continuous variables as mean ± SEM. All quantitative data were analyzed by pair comparisons, one way or repeated measure ANOVA. A p value of less than 0.05 was considered to be statistically significant.

Results

Effect of PL on collagen-induced platelet activation and aggregation

PL dose-dependently blocked collagen-induced platelet aggregation with a maximal inhibition achieved at 100 μM (Fig 1A). This inhibitory effect was observed at the subthreshold (2 μg/ml) and high (5 μg/ml) concentration of collagen, but not at a maximal concentration of 10 μg/ml (Fig 1B). PL was equally effective in blocking platelet thrombus formation on immobilized collagen under an arterial shear stress of 60 dynes/cm² (Fig 1C). Consistent with its effect on platelet aggregation and thrombus formation, PL partially blocked the collagen-induced expression of CD62p (Fig 1D), binding of PAC-1, an antibody that specifically recognizes the activated form of the integrin αIIbβ3 (Fig 1E) and calcium influx (Fig 1F). These inhibitory activities of PL were not mediated by inducing receptor shedding because surface densities of GP VI (Fig 2A), which were reduced by collagen stimulation, and the integrin αIIbß₃ (Fig 2B) were not reduced by the PL treatment. As control, collagen induced a significant increase in the expression of integrin αIIbß₃. PL also inhibited platelet aggregation induced by CRP (Fig 2C), which specifically targets GP VI, one of two collagen receptors on platelets. In contrast, PL had no effect on collagen-induced aggregation of platelets from mice deficient in platelet STAT3 (S1 Fig). Aggregation of human platelets by ADP (5 μM) and TRAP (50 μM), pretreated with PL also induced aggregation at a level comparable to 5 μg/ml of collagen (S2 Fig).

Download:

Fig 1. PL inhibited collagen-induced platelet reactivity.

(A) Platelets were induced to aggregate by 5 μg/ml of collagen in the presence of increasing concentrations of PL (a representative of 10 separate experiments). (B) PL blocked platelet aggregation induced by low doses, but not a maximal dose of collagen (n = 10, paired t test). (C) PL blocked the thrombus formation of platelets on the collagen matrix under flow conditions (panels a-e are representative images [bar = 100 μm] and panel f is a summary of 6 separate experiments, repeated measures ANOVA, * p < 0.01 compared untreated platelets). PL blocked collagen-induced CD62p expression (D), PAC-1 binding (E), and calcium influx (F). Data presented in panels D-F were obtained from 6–8 donors and analyzed by ANOVA (panels D-E) and t test (panel F).

https://doi.org/10.1371/journal.pone.0143964.g001

Download:

Fig 2. Effects of PL on collagen-induced platelet activation, morphological transition, and microvesiculation.

PRP was stimulated with 5 μg/ml of collagen in the presence and absence of 100 μM PL. Surface expressions of GP VI (A, n = 5, ANOVA) and αIIbßß₃ (B, n = 6, * p < 0.001 compared to PL treated platelets) were measured by flow cytometry using specific monoclonal antibodies. (C) PL dose-dependently blocked CRP-induced platelet aggregation (n = 6, ANOVA). The morphological transition of adherent platelets on the collagen matrix was monitored by HPICM over ~60 min (D & E, bar = 10 μm). A ratio of HDBS to LDSS platelets was calculated (F, n = 6, paired t test) and CD42b⁺ and annexin V⁺ platelet microparticles were quantified (G, n = 6, paired t test).

https://doi.org/10.1371/journal.pone.0143964.g002

Effect of PL on collagen-induced microparticle production.

We previously used a novel HPICM technology to monitor ADP-induced morphological changes and microvesiculation of adherent platelets on immobilized fibrinogen [24]. This technology was modified to monitor real time morphological transformations and microparticle production of platelets on immobilized collagen. As shown in Fig 2D, platelets adherent to collagen presented as predominantly high density bubble shapes (HDBS), which we previously found to be sensitive to agonist-induced microvesiculation [24]. In contrast, many of the PL-treated platelets underwent a reverse transformation from a high-density bubble shape to a low-density spread shape (LDSS, Fig 2E), resulting in a significantly reduced ratio of HDBS to LDSS platelets (Fig 2F) and a reduced production of platelet microparticles (Fig 2G). Together, data presented in Figs 1 and 2 demonstrated an inhibitory activity of PL towards collagen-induced platelet activation and aggregation.

Effect of PL on collagen-induced STAT3 activation.

We have recently shown that PL potently inhibits STAT3 activation in cancer cells [19] and that STAT3 non-transcriptionally regulates collagen-induced platelet activation/aggregation by facilitating an interaction between the kinase Syk and the substrate PLCγ2 [22]. These results led us to hypothesize that PL targets STAT3 to block collagen-induced platelet reactivity. Here, we provide several lines of experimental evidence to support the hypothesis. First, PL blocked the tyrosine phosphorylation of JAK2 (Fig 3A) and STAT3 (Fig 3B) in platelets stimulated with collagen. As a control, STAT3 phosphorylation induced by a complex of IL-6-sIL-6Rα, which signals through the JAK2-STAT3 pathway in eliciting an acute phase reaction, was also blocked by PL (Fig 3B). Second, PL was significantly less effective in platelets pretreated with the STAT3 inhibitor STA21 (Fig 3C), whereas its effect was additive to that of the transcription inhibitor Actinomycin D (Fig 3D). The latter result suggests that PL acted independent of (mitochondrial) transcription in platelets. Third, the JAK2 inhibitor AG490 dose-dependently blocked collagen-induced platelet aggregation (Fig 3E) and thrombus formation on a collagen matrix under an arterial fluid shear stress of 60 dynes/cm² (Fig 3F).

Download:

Fig 3. PL blocked JAK2-STAT3 activation.

Lysates of platelets stimulated with collagen in the presence of PL were probed for total and phospho-JAK2 (A) and STAT3 (B). STAT3 phosphorylation was also probed in platelets treated with a complex of IL-6-sIL-6α either alone or combined with collagen as control (B). Platelet aggregation was also induced by collagen in the presence of a submaximal 50 μM of PL with and without a maximal inhibitory 50 μM of STA21 (C, a representative of 6 experiments) or actinomycin D (D, a representative of 6 experiments). Platelets treated with an increasing concentration of the JAK2 inhibitor AG490 were induced to aggregate (E) and to form thrombi on immobilized collagen under flow condition (F, bar = 100 μm, the panel e summaries results from 3 experiments, repeated measure ANOVA, *p < 0.01).

https://doi.org/10.1371/journal.pone.0143964.g003

While PL did not inhibit the tyrosine phosphorylation of Syk (Fig 4A), it was effective in blocking PLCγ2 phosphorylation (Fig 4B) in collagen-stimulated platelets. This regulatory profile of PL is identical to that of STAT3 inhibitors on platelets [22], suggesting that PL does not directly inhibit GP VI-mediated signaling, but disrupts the phosphorylation and subsequent dimerization of STAT3, which are necessary to accelerate or enhance the activity of Syk kinase towards the substrate PLCγ2. Consistent with this notion, the Syk inhibitor SykII inhibited collagen-induced platelet aggregation in synergy with the inhibitory activity of PL (Fig 4C).

Download:

Fig 4. PL effect on collagen-GP VI signaling.

Lysates of platelets treated with collagen in the presence of PL were probed for total and phosphorylated Syk (A) and PLCγ2 (B). (C) Platelets were first incubated with SykII for 10 min followed by additional 10 min incubation with PL before being stimulated with collagen (n = 3, repeated measures ANOVA, *p < 0.01).

https://doi.org/10.1371/journal.pone.0143964.g004

Differential ROS production in platelets treated with PL or collagen.

Collagen has been reported to induce ROS release from platelets [18] and several varieties of ROS are known to activate platelets [25], suggesting that ROS is stimulatory to platelets. However, PL has been shown to induce ROS production in cancerous, but not normal cells by binding and down-regulating the activities of GSTP1 and carbonyl reductase 1 CBR1 [11]. These contradictory observations prompted us to examine whether PL induces ROS in platelets. PL at 100 μM that maximally blocked collagen-induced platelet activation and aggregation (Fig 1) induced the release of ROS in platelets as detected by flow cytometry using DCFH-DA and CellRox Red probes (Fig 5A). GSTP1 and CBR1 were also detected in platelets at levels that were not altered by collagen-or/and IL-6-sIL-6α stimulations (S3 Fig). Consistent with previous reports [18], collagen induced platelet production of ROS in a dose dependent manner and its effect was additive to that of PL (Fig 5B). This potent effect of PL on ROS production was further validated by a significant reduction of free GSH in platelets treated with PL, but not with collagen (Fig 5C). However, quenching ROS with 20 μM of cell non-permeable GSH (Fig 5D) or 0.5 mM of cell permeable L-Cysteine (Fig 5E) did not reverse the inhibitory effects of PL on collagen-induced platelet aggregation, even though both anti-oxidants were used at concentrations significantly higher than their baseline plasma levels [26;27]. GSH also failed to reverse PL-induced reduction of PAC-1 binding to collagen-stimulated platelets (Fig 5G). Apocynin, which is an inhibitor of the reduced nicotinamide adenine dinucleotide phosphate (NADPH) oxidase and reported to block collagen-induced ROS production in platelets [18] did not alter the effect of PL on collagen-induced platelet aggregation (Fig 5H).

Download:

Fig 5. PL-induced ROS production and activity.

Platelets in PRP were labeled with either CellROX Red or DCFH-DA for 30 min at 37°C and treated with either100 μM of PL or vehicle control (BL) for additional 10 min. ROS production was measured in platelets by flow cytometry (A, n = 10, paired t test). ROS production was also measured in platelets stimulated with various doses of collagen in the presence and absence of PL (B, n = 6, paired t test). Free GSH was measured by mass spectrometry in resting platelets and those treated with either PL or collagen for 10 min at 37°C (C, n = 3, one way ANOVA). Collagen-induced aggregation was recorded in platelets preincubated with either GSH (D) or L-cysteine before treatment with 100 μM PL (E). Platelets treated with GSH or L-cysteine without PL were tested as controls (panel F summaries data from 3 experiments). Platelets were treated with collagen, PL, and PL plus GSH for 10 min at 37°C. PAC-1 binding was then detected by flow cytometry (G, a representative of 3 experiments). PRP was incubated with Apocynin for 10 min at 37°C followed by additional 10 min of incubation with 100 μM of PL. Collagen-induced platelet aggregation was then recorded (H, a representative of 3 experiments).

https://doi.org/10.1371/journal.pone.0143964.g005

Generation and testing of synthetic analogs.

The diverse effects of PL on cancer cells and platelets may result from different structures and chemical moieties. To examine the role of specific chemical moieties in blocking platelet reactivity to collagen, we synthesized two PL analogs (Fig 6A) through hydrogeneration [3] and by introducing a terminal alkyne [11] at a site away from the possible “bioactivity bearing” functional groups (compound 1 & 2). The two derivatives were found to be active in blocking platelet aggregation induced by 2 μg/ml (Fig 6B and 6D), but not at 5 μg/ml of collagen (data not shown).

Download:

Fig 6. Effects of PL analogs on collagen-induced platelet aggregation.

(A) PL and structural derivatives compound 1 (C1) and compound 2 (C2). (B) PRP was incubated with PL, C1 or C2 for 15 min at 37°C and then induced to aggregate by 2 μg/ml of collagen (a representative of 10 experiments). (C & D) C1 and C2 were also tested at different doses for their impact on collagen-induced platelet aggregation.

https://doi.org/10.1371/journal.pone.0143964.g006

Discussion

PL has been reported to be inhibitory to several major platelet agonists. Here, we have specifically characterized inhibitory effects of PL on collagen-induced platelet reactivity (Figs 1 and 2) to explore the influence of PL on the platelet JAK2- STAT3 pathway. Our findings are consistent with previous reports [13;14]. We have also made several new observations that define the mechanism by which PL inhibits collagen-induced platelet activation and provide new information regarding the differential effects of ROS on platelet reactivity to collagen.

First, PL inhibited collagen-induced platelet reactivity primarily by blocking the activation of JAK2 and STAT3. This conclusion is supported by several lines of experimental evidence presented in Figs 3 & 4. In nucleated cells, tyrosine phosphorylated STAT3 dimerizes to be more efficiently translocated into the nucleus to regulate the transcription of multiple genes associated with the acute phase reaction [28–31]. We have recently shown that a STAT3 dimer enhances collagen-induced signaling in platelets by serving as a protein scaffold for Syk and PLCγ2 [22] and PL prevents this critical dimerization by preventing JAK2-mediated STAT2 activation [19]. Furthermore, PL did not directly inhibit collagen-induced Syk phosphorylation, but did block the activation of its substrate PLCγ2. This regulatory profile is consistent with the notion that a phosphorylated STAT3 dimer serving as a protein scaffold linking the kinase Syk to the substrate PLCγ2 in the GP IV signal pathway. Furthermore, the JAK2 inhibitor AG-490 (Tyrphostin B42), which has no effect on the kinases Lyn, Syk and Src involved in GP VI signaling, also blocked collagen-induced platelet aggregation and thrombus formation under flow conditions (Fig 3E and 3F). Together, these data suggest that PL directly prevents STAT3 dimerization and indirectly by blocking JAK2 activation.

Second, both PL and collagen induced ROS production in platelets (Fig 5A–5C), but PL’s inhibitory activity on collagen-induced platelet activation was not affected by the ROS (Fig 5D–5G). The results raise two interesting questions. The first regards the previous reports that PL induces ROS production by inhibiting GSTP1 activity specifically in cancerous, but not normal cells, leading to ROS-mediated apoptosis [3;11]. Platelets treated with PL did not undergo apoptosis as they remained aggregatable in response to high doses of collagen (Fig 1B), ADP (S1 Fig) and TRAP (S1 Fig). They also had a reduced rate of microvesiculation (Fig 2E–2H). The second question regards the impact of ROS on platelet reactivity. The inhibitory effects of PL on collagen-induced platelet reactivity was not affected by cell permeable and non-permeable reducing agents that quench extracellular and intracellular oxidants; and by a NADPH oxidase inhibitor (Fig 5D–5G), which blocked collagen-and thrombin-induced ROS production in platelets [17;18]. The finding strongly suggests that PL and collagen induce the release of different oxidants that have differential effects on platelets. For example, PL induces cancer cells to produce nitric oxide [11], which is a well-known platelet inhibitor [32]. Our finding also differs from the reported effect of the GSH precursor N-acetyl-L-cysteine on eliminating PL’s effect on cancer cells [11], implying that PL acts differently in cancer cells and in platelets. Studying these differential effects on drug-induced oxidative stress may uncover new mechanisms of regulating platelet functions by selective oxidants.

Third, we made and tested two PL analogs with specific structure modifications. These analogs are designed to help differentiate the contributions of specific structures on inhibitory activity of PL in collagen-induced platelet reactivity. The double bonds C3-C4 and C7-C8 in PL were reduced in compound 1 to make the analog less reactive. It has also been shown that the electrophilicity of the C2-C3 olefin is critical for the apoptotic effects of PL on cancer cells, whereas analogs lacking a reactive C7-C8 olefin induce intracellular ROS, but markedly reduced cell death [3]. In contrast, compound 2 was designed as a potential probe to identify biological targets of PL and to provide structure-activity relationships. However, both derivatives are equally active in blocking platelet reactivity to the low dose of collagen (Fig 6).

In summary, we have shown that PL inhibits collagen-induced platelet activation, aggregation, and thrombus formation by primarily blocking JAK2-STAT3 phosphorylation, reducing the ability of STAT3 to serve as a protein scaffold for linking Syk to PLCγ2. We further show that, while PL induces ROS in platelets, its inhibitory activity towards collagen-induced platelet activation was not affected by ROS, suggesting that ROS have differential effects on platelet reactivity.

Supporting Information

S1 Fig. Citrated PRP from STAT3^-/- and littermate control mice were preincubated with either PL and the vehicle DMSO for 10 min at 37°C and then stimulated with 0.75 μg/ml of fibrillary type I collagen.

Platelet aggregation was monitored for 10 min at 37°C. We have previously shown that, at this dose of collagen, the collagen-induced aggregation of platelet from STAT3^-/- was significantly reduced as compared to control platelets (22). Here, we further show that PL was not active in blocking collagen-induced aggregation of platelets from the STAT3^-/- mice (n = 8 mice/group, paired t test).

https://doi.org/10.1371/journal.pone.0143964.s001

(JPG)

S2 Fig. Platelet aggregation induced by 5 μM of ADP (A) or 50 μM of TRAP (B) was not blocked by PL.

https://doi.org/10.1371/journal.pone.0143964.s002

(JPG)

S3 Fig. Expression of GSTP-1 and CBR-1 in platelets detected by immunoblots.

https://doi.org/10.1371/journal.pone.0143964.s003

(JPG)

Acknowledgments

We thank the Vice President for Research, College of Science, and Department of Chemistry at Texas A&M University for seed funding to the Natural Products LINCHPIN Laboratory.

Author Contributions

Conceived and designed the experiments: DJT DR XF JZ JFD. Performed the experiments: HY KLH YT UB XW ZZ MZ. Analyzed the data: HY KLH YT UB XW YZ. Contributed reagents/materials/analysis tools: KH. Wrote the paper: DJT DR XF JZ JFD.

References

1. Kumar S, Kamboj J, Suman , Sharma S. 2011. Overview for various aspects of the health benefits of Piper longum linn. fruit. J. Acupunct. Meridian. Stud. 4:134–140. pmid:21704957
- View Article
- PubMed/NCBI
- Google Scholar
2. Bezerra DP, Pessoa C, de Moraes MO, Saker-Neto N, Silveira ER, Costa-Lotufo LV. 2012. Overview of the therapeutic potential of piplartine (piperlongumine). Eur. J. Pharm. Sci. 48:453–463. pmid:23238172
- View Article
- PubMed/NCBI
- Google Scholar
3. Adams DJ, Dai M, Pellegrino G, Wagner BK, Stern AM, Shamji AF, et al. 2012. Synthesis, cellular evaluation, and mechanism of action of piperlongumine analogs. Proc. Natl. Acad. Sci. U. S. A. 109:15115–15120. pmid:22949699
- View Article
- PubMed/NCBI
- Google Scholar
4. Morikawa T, Matsuda H, Yamaguchi I, Pongpiriyadacha Y, Yoshikawa M. 2004. New amides and gastroprotective constituents from the fruit of Piper chaba. Planta Med. 70:152–159. pmid:14994194
- View Article
- PubMed/NCBI
- Google Scholar
5. Silva DR, Endo EH, Filho BP, Nakamura CV, Svidzinski TI, de SA, et al. 2009. Chemical Composition and Antimicrobial Properties of Piper ovatum Vahl. Molecules. 14:1171–1182. pmid:19325517
- View Article
- PubMed/NCBI
- Google Scholar
6. Lee SE, Park BS, Bayman P, Baker JL, Choi WS, Campbell BC. 2007. Suppression of ochratoxin biosynthesis by naturally occurring alkaloids. Food Addit. Contam. 24:391–397. pmid:17454112
- View Article
- PubMed/NCBI
- Google Scholar
7. Zhang H, Matsuda H, Nakamura S, Yoshikawa M. 2008. Effects of amide constituents from pepper on adipogenesis in 3T3-L1 cells. Bioorg. Med. Chem. Lett. 18:3272–3277. pmid:18477507
- View Article
- PubMed/NCBI
- Google Scholar
8. Jin Z, Borjihan G, Zhao R, Sun Z, Hammond GB, Uryu T. 2009. Antihyperlipidemic compounds from the fruit of Piper longum L. Phytother. Res. 23:1194–1196. pmid:19172581
- View Article
- PubMed/NCBI
- Google Scholar
9. Son DJ, Kim SY, Han SS, Kim CW, Kumar S, Park BS, et al. 2012. Piperlongumine inhibits atherosclerotic plaque formation and vascular smooth muscle cell proliferation by suppressing PDGF receptor signaling. Biochem. Biophys. Res. Commun. 19;427:349–354. pmid:22995306
- View Article
- PubMed/NCBI
- Google Scholar
10. Kim KS, Kim JA, Eom SY, Lee SH, Min KR, Kim Y. 2006. Inhibitory effect of piperlonguminine on melanin production in melanoma B16 cell line by downregulation of tyrosinase expression. Pigment Cell Res. 19:90–98. pmid:16420250
- View Article
- PubMed/NCBI
- Google Scholar
11. Raj L, Ide T, Gurkar AU, Foley M, Schenone M, Li X, et al. 2011. Selective killing of cancer cells by a small molecule targeting the stress response to ROS. Nature. 475:231–234. pmid:21753854
- View Article
- PubMed/NCBI
- Google Scholar
12. Jarvius M, Fryknas M, D'Arcy P, Sun C, Rickardson L, Gullbo J, et al. 2013. Piperlongumine induces inhibition of the ubiquitin-proteasome system in cancer cells. Biochem. Biophys. Res. Commun. 431:117–123. pmid:23318177
- View Article
- PubMed/NCBI
- Google Scholar
13. Park BS, Son DJ, Choi WS, Takeoka GR, Han SO, Kim TW, et al. 2008. Antiplatelet activities of newly synthesized derivatives of piperlongumine. Phytother. Res. 22:1195–1199. pmid:18697182
- View Article
- PubMed/NCBI
- Google Scholar
14. Park BS, Son DJ, Park YH, Kim TW, Lee SE. 2007. Antiplatelet effects of acidamides isolated from the fruits of Piper longum L. Phytomedicine. 14:853–855. pmid:17689230
- View Article
- PubMed/NCBI
- Google Scholar
15. Iwashita M, Oka N, Ohkubo S, Saito M, Nakahata N. 2007. Piperlongumine, a constituent of Piper longum L., inhibits rabbit platelet aggregation as a thromboxane A(2) receptor antagonist. Eur. J. Pharmacol. 570:38–42. pmid:17618620
- View Article
- PubMed/NCBI
- Google Scholar
16. Arthur JF, Gardiner EE, Kenny D, Andrews RK, Berndt MC. 2008. Platelet receptor redox regulation. Platelets. 19:1–8. pmid:18231933
- View Article
- PubMed/NCBI
- Google Scholar
17. Begonja AJ, Gambaryan S, Geiger J, Aktas B, Pozgajova M, Nieswandt B, et al. 2005. Platelet NAD(P)H-oxidase-generated ROS production regulates alphaIIbbeta3-integrin activation independent of the NO/cGMP pathway. Blood. 106:2757–2760. pmid:15976180
- View Article
- PubMed/NCBI
- Google Scholar
18. Arthur JF, Qiao J, Shen Y, Davis AK, Dunne E, Berndt MC, et al. 2012. ITAM receptor-mediated generation of reactive oxygen species in human platelets occurs via Syk-dependent and Syk-independent pathways. J. Thromb. Haemost. 10:1133–1141. pmid:22489915
- View Article
- PubMed/NCBI
- Google Scholar
19. Bharadwaj U, Eckols TK, Kolosov M, Kasembeli MM, Adam A, Torres D, et al. 2014. Drug-repositioning screening identified piperlongumine as a direct STAT3 inhibitor with potent activity against breast cancer. Oncogene (in press).
- View Article
- Google Scholar
20. Mieyal JJ, Chock PB. 2012. Posttranslational modification of cysteine in redox signaling and oxidative stress: Focus on s-glutathionylation. Antioxid. Redox. Signal. 16:471–475. pmid:22136616
- View Article
- PubMed/NCBI
- Google Scholar
21. Zhong Z, Wen Z, Darnell JE Jr. 1994. Stat3: a STAT family member activated by tyrosine phosphorylation in response to epidermal growth factor and interleukin-6. Science. 264:95–98. pmid:8140422
- View Article
- PubMed/NCBI
- Google Scholar
22. Zhou Z, Gushiken FC, Bolgiano D, Salsbery BJ, Aghakasiri N, Jing N, et al. 2013. Signal transducer and activator of transcription 3 (STAT3) regulates collagen-induced platelet aggregation independently of its transcription factor activity. Circulation. 127:476–485. pmid:23266857
- View Article
- PubMed/NCBI
- Google Scholar
23. Hu H, Forslund M, Li N. 2005. Influence of extracellular calcium on single platelet activation as measured by whole blood flow cytometry. Thromb. Res. 116:241–247. pmid:15935833
- View Article
- PubMed/NCBI
- Google Scholar
24. Zhang Y, Liu X, Liu L, Zaske AM, Zhou Z, Fu Y, et al. 2013. Contact- and agonist-regulated microvesiculation of human platelets. Thromb. Haemost. 110:331–339. pmid:23784603
- View Article
- PubMed/NCBI
- Google Scholar
25. Bosin TR, Schaltenbrand SL. 1991. Stimulation of platelet serotonin transport by substituted 1,4-naphthoquinone-induced oxidant stress. Biochem. Pharmacol. 41:967–974. pmid:1848980
- View Article
- PubMed/NCBI
- Google Scholar
26. Milsom JP, Morgan MY, Sherlock S. 1979. Factors affecting plasma amino acid concentrations in control subjects. Metabolism. 28:313–319. pmid:571951
- View Article
- PubMed/NCBI
- Google Scholar
27. Essex DW, and Li M. 2003. Redox control of platelet aggregation. Biochemistry. 42:129–136. pmid:12515547
- View Article
- PubMed/NCBI
- Google Scholar
28. Wegenka UM, Buschmann J, Lutticken C, Heinrich PC, Horn F. 1993. Acute-phase response factor, a nuclear factor binding to acute-phase response elements, is rapidly activated by interleukin-6 at the posttranslational level. Mol. Cell Biol 13:276–288. pmid:7678052
- View Article
- PubMed/NCBI
- Google Scholar
29. Lutticken C, Wegenka UM, Yuan J, Buschmann J, Schindler C, Ziemiecki A, et al. 1994. Association of transcription factor APRF and protein kinase Jak1 with the interleukin-6 signal transducer gp130. Science 263:89–92. pmid:8272872
- View Article
- PubMed/NCBI
- Google Scholar
30. Wen Z, Zhong Z, Darnell JE Jr. 1995. Maximal activation of transcription by Stat1 and Stat3 requires both tyrosine and serine phosphorylation. Cell. 82:241–250. pmid:7543024
- View Article
- PubMed/NCBI
- Google Scholar
31. Reich NC, Liu L. 2006. Tracking STAT nuclear traffic. Nat. Rev. Immunol. 6:602–612. pmid:16868551
- View Article
- PubMed/NCBI
- Google Scholar
32. Gkaliagkousi E, Ritter J, Ferro A. 2007. Platelet-derived nitric oxide signaling and regulation. Circ. Res. 101:654–662. pmid:17901370
- View Article
- PubMed/NCBI
- Google Scholar

[ref1] 1. Kumar S, Kamboj J, Suman , Sharma S. 2011. Overview for various aspects of the health benefits of Piper longum linn. fruit. J. Acupunct. Meridian. Stud. 4:134–140. pmid:21704957
View Article
PubMed/NCBI
Google Scholar

[2] View Article

[3] PubMed/NCBI

[4] Google Scholar

[ref2] 2. Bezerra DP, Pessoa C, de Moraes MO, Saker-Neto N, Silveira ER, Costa-Lotufo LV. 2012. Overview of the therapeutic potential of piplartine (piperlongumine). Eur. J. Pharm. Sci. 48:453–463. pmid:23238172
View Article
PubMed/NCBI
Google Scholar

[6] View Article

[7] PubMed/NCBI

[8] Google Scholar

[ref3] 3. Adams DJ, Dai M, Pellegrino G, Wagner BK, Stern AM, Shamji AF, et al. 2012. Synthesis, cellular evaluation, and mechanism of action of piperlongumine analogs. Proc. Natl. Acad. Sci. U. S. A. 109:15115–15120. pmid:22949699
View Article
PubMed/NCBI
Google Scholar

[10] View Article

[11] PubMed/NCBI

[12] Google Scholar

[ref4] 4. Morikawa T, Matsuda H, Yamaguchi I, Pongpiriyadacha Y, Yoshikawa M. 2004. New amides and gastroprotective constituents from the fruit of Piper chaba. Planta Med. 70:152–159. pmid:14994194
View Article
PubMed/NCBI
Google Scholar

[14] View Article

[15] PubMed/NCBI

[16] Google Scholar

[ref5] 5. Silva DR, Endo EH, Filho BP, Nakamura CV, Svidzinski TI, de SA, et al. 2009. Chemical Composition and Antimicrobial Properties of Piper ovatum Vahl. Molecules. 14:1171–1182. pmid:19325517
View Article
PubMed/NCBI
Google Scholar

[18] View Article

[19] PubMed/NCBI

[20] Google Scholar

[ref6] 6. Lee SE, Park BS, Bayman P, Baker JL, Choi WS, Campbell BC. 2007. Suppression of ochratoxin biosynthesis by naturally occurring alkaloids. Food Addit. Contam. 24:391–397. pmid:17454112
View Article
PubMed/NCBI
Google Scholar

[22] View Article

[23] PubMed/NCBI

[24] Google Scholar

[ref7] 7. Zhang H, Matsuda H, Nakamura S, Yoshikawa M. 2008. Effects of amide constituents from pepper on adipogenesis in 3T3-L1 cells. Bioorg. Med. Chem. Lett. 18:3272–3277. pmid:18477507
View Article
PubMed/NCBI
Google Scholar

[26] View Article

[27] PubMed/NCBI

[28] Google Scholar

[ref8] 8. Jin Z, Borjihan G, Zhao R, Sun Z, Hammond GB, Uryu T. 2009. Antihyperlipidemic compounds from the fruit of Piper longum L. Phytother. Res. 23:1194–1196. pmid:19172581
View Article
PubMed/NCBI
Google Scholar

[30] View Article

[31] PubMed/NCBI

[32] Google Scholar

[ref9] 9. Son DJ, Kim SY, Han SS, Kim CW, Kumar S, Park BS, et al. 2012. Piperlongumine inhibits atherosclerotic plaque formation and vascular smooth muscle cell proliferation by suppressing PDGF receptor signaling. Biochem. Biophys. Res. Commun. 19;427:349–354. pmid:22995306
View Article
PubMed/NCBI
Google Scholar

[34] View Article

[35] PubMed/NCBI

[36] Google Scholar

[ref10] 10. Kim KS, Kim JA, Eom SY, Lee SH, Min KR, Kim Y. 2006. Inhibitory effect of piperlonguminine on melanin production in melanoma B16 cell line by downregulation of tyrosinase expression. Pigment Cell Res. 19:90–98. pmid:16420250
View Article
PubMed/NCBI
Google Scholar

[38] View Article

[39] PubMed/NCBI

[40] Google Scholar

[ref11] 11. Raj L, Ide T, Gurkar AU, Foley M, Schenone M, Li X, et al. 2011. Selective killing of cancer cells by a small molecule targeting the stress response to ROS. Nature. 475:231–234. pmid:21753854
View Article
PubMed/NCBI
Google Scholar

[42] View Article

[43] PubMed/NCBI

[44] Google Scholar

[ref12] 12. Jarvius M, Fryknas M, D'Arcy P, Sun C, Rickardson L, Gullbo J, et al. 2013. Piperlongumine induces inhibition of the ubiquitin-proteasome system in cancer cells. Biochem. Biophys. Res. Commun. 431:117–123. pmid:23318177
View Article
PubMed/NCBI
Google Scholar

[46] View Article

[47] PubMed/NCBI

[48] Google Scholar

[ref13] 13. Park BS, Son DJ, Choi WS, Takeoka GR, Han SO, Kim TW, et al. 2008. Antiplatelet activities of newly synthesized derivatives of piperlongumine. Phytother. Res. 22:1195–1199. pmid:18697182
View Article
PubMed/NCBI
Google Scholar

[50] View Article

[51] PubMed/NCBI

[52] Google Scholar

[ref14] 14. Park BS, Son DJ, Park YH, Kim TW, Lee SE. 2007. Antiplatelet effects of acidamides isolated from the fruits of Piper longum L. Phytomedicine. 14:853–855. pmid:17689230
View Article
PubMed/NCBI
Google Scholar

[54] View Article

[55] PubMed/NCBI

[56] Google Scholar

[ref15] 15. Iwashita M, Oka N, Ohkubo S, Saito M, Nakahata N. 2007. Piperlongumine, a constituent of Piper longum L., inhibits rabbit platelet aggregation as a thromboxane A(2) receptor antagonist. Eur. J. Pharmacol. 570:38–42. pmid:17618620
View Article
PubMed/NCBI
Google Scholar

[58] View Article

[59] PubMed/NCBI

[60] Google Scholar

[ref16] 16. Arthur JF, Gardiner EE, Kenny D, Andrews RK, Berndt MC. 2008. Platelet receptor redox regulation. Platelets. 19:1–8. pmid:18231933
View Article
PubMed/NCBI
Google Scholar

[62] View Article

[63] PubMed/NCBI

[64] Google Scholar

[ref17] 17. Begonja AJ, Gambaryan S, Geiger J, Aktas B, Pozgajova M, Nieswandt B, et al. 2005. Platelet NAD(P)H-oxidase-generated ROS production regulates alphaIIbbeta3-integrin activation independent of the NO/cGMP pathway. Blood. 106:2757–2760. pmid:15976180
View Article
PubMed/NCBI
Google Scholar

[66] View Article

[67] PubMed/NCBI

[68] Google Scholar

[ref18] 18. Arthur JF, Qiao J, Shen Y, Davis AK, Dunne E, Berndt MC, et al. 2012. ITAM receptor-mediated generation of reactive oxygen species in human platelets occurs via Syk-dependent and Syk-independent pathways. J. Thromb. Haemost. 10:1133–1141. pmid:22489915
View Article
PubMed/NCBI
Google Scholar

[70] View Article

[71] PubMed/NCBI

[72] Google Scholar

[ref19] 19. Bharadwaj U, Eckols TK, Kolosov M, Kasembeli MM, Adam A, Torres D, et al. 2014. Drug-repositioning screening identified piperlongumine as a direct STAT3 inhibitor with potent activity against breast cancer. Oncogene (in press).
View Article
Google Scholar

[74] View Article

[75] Google Scholar

[ref20] 20. Mieyal JJ, Chock PB. 2012. Posttranslational modification of cysteine in redox signaling and oxidative stress: Focus on s-glutathionylation. Antioxid. Redox. Signal. 16:471–475. pmid:22136616
View Article
PubMed/NCBI
Google Scholar

[77] View Article

[78] PubMed/NCBI

[79] Google Scholar

[ref21] 21. Zhong Z, Wen Z, Darnell JE Jr. 1994. Stat3: a STAT family member activated by tyrosine phosphorylation in response to epidermal growth factor and interleukin-6. Science. 264:95–98. pmid:8140422
View Article
PubMed/NCBI
Google Scholar

[81] View Article

[82] PubMed/NCBI

[83] Google Scholar

[ref22] 22. Zhou Z, Gushiken FC, Bolgiano D, Salsbery BJ, Aghakasiri N, Jing N, et al. 2013. Signal transducer and activator of transcription 3 (STAT3) regulates collagen-induced platelet aggregation independently of its transcription factor activity. Circulation. 127:476–485. pmid:23266857
View Article
PubMed/NCBI
Google Scholar

[85] View Article

[86] PubMed/NCBI

[87] Google Scholar

[ref23] 23. Hu H, Forslund M, Li N. 2005. Influence of extracellular calcium on single platelet activation as measured by whole blood flow cytometry. Thromb. Res. 116:241–247. pmid:15935833
View Article
PubMed/NCBI
Google Scholar

[89] View Article

[90] PubMed/NCBI

[91] Google Scholar

[ref24] 24. Zhang Y, Liu X, Liu L, Zaske AM, Zhou Z, Fu Y, et al. 2013. Contact- and agonist-regulated microvesiculation of human platelets. Thromb. Haemost. 110:331–339. pmid:23784603
View Article
PubMed/NCBI
Google Scholar

[93] View Article

[94] PubMed/NCBI

[95] Google Scholar

[ref25] 25. Bosin TR, Schaltenbrand SL. 1991. Stimulation of platelet serotonin transport by substituted 1,4-naphthoquinone-induced oxidant stress. Biochem. Pharmacol. 41:967–974. pmid:1848980
View Article
PubMed/NCBI
Google Scholar

[97] View Article

[98] PubMed/NCBI

[99] Google Scholar

[ref26] 26. Milsom JP, Morgan MY, Sherlock S. 1979. Factors affecting plasma amino acid concentrations in control subjects. Metabolism. 28:313–319. pmid:571951
View Article
PubMed/NCBI
Google Scholar

[101] View Article

[102] PubMed/NCBI

[103] Google Scholar

[ref27] 27. Essex DW, and Li M. 2003. Redox control of platelet aggregation. Biochemistry. 42:129–136. pmid:12515547
View Article
PubMed/NCBI
Google Scholar

[105] View Article

[106] PubMed/NCBI

[107] Google Scholar

[ref28] 28. Wegenka UM, Buschmann J, Lutticken C, Heinrich PC, Horn F. 1993. Acute-phase response factor, a nuclear factor binding to acute-phase response elements, is rapidly activated by interleukin-6 at the posttranslational level. Mol. Cell Biol 13:276–288. pmid:7678052
View Article
PubMed/NCBI
Google Scholar

[109] View Article

[110] PubMed/NCBI

[111] Google Scholar

[ref29] 29. Lutticken C, Wegenka UM, Yuan J, Buschmann J, Schindler C, Ziemiecki A, et al. 1994. Association of transcription factor APRF and protein kinase Jak1 with the interleukin-6 signal transducer gp130. Science 263:89–92. pmid:8272872
View Article
PubMed/NCBI
Google Scholar

[113] View Article

[114] PubMed/NCBI

[115] Google Scholar

[ref30] 30. Wen Z, Zhong Z, Darnell JE Jr. 1995. Maximal activation of transcription by Stat1 and Stat3 requires both tyrosine and serine phosphorylation. Cell. 82:241–250. pmid:7543024
View Article
PubMed/NCBI
Google Scholar

[117] View Article

[118] PubMed/NCBI

[119] Google Scholar

[ref31] 31. Reich NC, Liu L. 2006. Tracking STAT nuclear traffic. Nat. Rev. Immunol. 6:602–612. pmid:16868551
View Article
PubMed/NCBI
Google Scholar

[121] View Article

[122] PubMed/NCBI

[123] Google Scholar

[ref32] 32. Gkaliagkousi E, Ritter J, Ferro A. 2007. Platelet-derived nitric oxide signaling and regulation. Circ. Res. 101:654–662. pmid:17901370
View Article
PubMed/NCBI
Google Scholar

[125] View Article

[126] PubMed/NCBI

[127] Google Scholar

Piperlongumine Blocks JAK2-STAT3 to Inhibit Collagen-Induced Platelet Reactivity Independent of Reactive Oxygen Species^†

Piperlongumine Blocks JAK2-STAT3 to Inhibit Collagen-Induced Platelet Reactivity Independent of Reactive Oxygen Species^†

Correction

Figures

Abstract

Background

Objective

Results

Conclusions

Introduction

Materials and Methods

Reagents

Methods

Platelet aggregation.

Platelet activation.

Hopping Probe Ion Conductance Microscopy imaging.

Measurement of platelet microparticles.

PL on thrombus formation.

Immunoblots.

Effect of PL on ROS production.

PL derivatives.

Statistical analyses.

Results

Effect of PL on collagen-induced platelet activation and aggregation

Effect of PL on collagen-induced microparticle production.

Effect of PL on collagen-induced STAT3 activation.

Differential ROS production in platelets treated with PL or collagen.

Generation and testing of synthetic analogs.

Discussion

Supporting Information

S1 Fig. Citrated PRP from STAT3^-/- and littermate control mice were preincubated with either PL and the vehicle DMSO for 10 min at 37°C and then stimulated with 0.75 μg/ml of fibrillary type I collagen.

S2 Fig. Platelet aggregation induced by 5 μM of ADP (A) or 50 μM of TRAP (B) was not blocked by PL.

S3 Fig. Expression of GSTP-1 and CBR-1 in platelets detected by immunoblots.

Acknowledgments

Author Contributions

References

Correction

Figures

Abstract

Background

Objective

Results

Conclusions

Introduction

Materials and Methods

Reagents

Methods

Platelet aggregation.

Platelet activation.

Hopping Probe Ion Conductance Microscopy imaging.

Measurement of platelet microparticles.

PL on thrombus formation.

Immunoblots.

Effect of PL on ROS production.

PL derivatives.

Statistical analyses.

Results

Effect of PL on collagen-induced platelet activation and aggregation

Effect of PL on collagen-induced microparticle production.

Effect of PL on collagen-induced STAT3 activation.

Differential ROS production in platelets treated with PL or collagen.

Generation and testing of synthetic analogs.

Discussion

Supporting Information

S1 Fig. Citrated PRP from STAT3-/- and littermate control mice were preincubated with either PL and the vehicle DMSO for 10 min at 37°C and then stimulated with 0.75 μg/ml of fibrillary type I collagen.

S2 Fig. Platelet aggregation induced by 5 μM of ADP (A) or 50 μM of TRAP (B) was not blocked by PL.

S3 Fig. Expression of GSTP-1 and CBR-1 in platelets detected by immunoblots.

Acknowledgments

Author Contributions

References

S1 Fig. Citrated PRP from STAT3^-/- and littermate control mice were preincubated with either PL and the vehicle DMSO for 10 min at 37°C and then stimulated with 0.75 μg/ml of fibrillary type I collagen.