Research Article | Open Access
Anna Zhang, Yunfeng Hou, Chao Sun, Ying Pu, Yu Sun, Yuan Zhang, Yang Shen, Qingbo Zhou, "Baicalin Protects against Thrombin-Induced Cell Injury in Human Umbilical Vein Endothelial Cells", BioMed Research International, vol. 2019, Article ID 2187306, 8 pages, 2019. https://doi.org/10.1155/2019/2187306
Baicalin Protects against Thrombin-Induced Cell Injury in Human Umbilical Vein Endothelial Cells
Thrombin plays a pivotal role in the pathogenesis of atherosclerosis. Baicalin, an active flavonoid compound, was shown to attenuate the development of atherosclerosis, but the mechanism remains elusive. In the present study, the role and mechanism of baicalin in thrombin-induced cell injury was investigated in human umbilical vein endothelial cells (HUVECs). Our results showed that baicalin significantly reduced thrombin-induced apoptosis of HUVECs. Additional experiments showed that baicalin inhibited thrombin-induced NF-κB activation and PAR-1 expression. In addition, baicalin decreased thrombin-induced PAR-1 expression by inhibiting ERK pathway. These results indicated that baicalin has protective effects on thrombin-induced cell injury in HUVECs possibly through inhibition of PAR-1 expression and its downstream NF-κB activation, which was mediated by ERK1/2 activation.
Atherosclerosis is the major cause of cardiovascular disease (CVD). Although great progress has been made, the incidence of CVD is increasing and the patients with atherosclerosis are becoming younger . Since 1990, CVD has become the leading cause of death in China .
The development of atherosclerosis involves in a variety of biological processes, including vascular endothelial cell injury, dyslipidemia, macrophage and T cell infiltration, smooth muscle cell hyperplasia, and thrombosis. Recently, accumulating evidence suggested that thrombin may play a pivotal role in the pathogenesis of atherosclerosis via damage of vascular endothelial cells .
Thrombin is produced by the enzymatic cleavage of two sites on prothrombin. Thrombin interacts with its specific cell membrane receptors (protease activated receptors: PAR-1, PAR-3, and PAR-4) which are abundantly expressed in all arterial vessel wall constituents, to participate in a number of biological processes, such as inflammation, leukocyte recruitment, oxidative stress, migration, and proliferation of vascular smooth muscle cells, cell apoptosis, and angiogenesis [3–5]. Transcription factor NF-κB plays an essential role in inflammation. NF-κB was shown to be activated upon thrombin stimulation and contributed to cell injury [6, 7].
Baicalin (7-glucuronic acid, 5, 6-dihydroxyflavone) is an active flavonoid compound, which is isolated from the medicinal plant Scutellaria baicalensis Georgi. It possesses many biological properties including antioxidant, antiplatelet, antithrombotic, and anticarcinogenic activities [8, 9]. Therefore, baicalin has been widely used for treatment of inflammatory diseases, such as asthma, nephritis, hepatitis, bronchitis, atopic dermatitis, and acute ischemic cerebrovascular diseases [10–12]. Our previous studies showed that baicalin had protective effects on SH-SY5Y cells against thrombin-induced cell injury through inhibiting the expression of PAR-1, MMP-9, and NMDA-R1  and attenuated focal cerebral ischemia reperfusion injury in an acute cerebral ischemia rat model . Additionally, baicalin was also suggested to ameliorate atherosclerosis possibly through lipid regulation, immune regulation, or activation of Wnt signaling pathway [15–17]. However, it is unclear whether baicalin has a protective effect on thrombin-induced cell injury in human umbilical vein endothelial cells (HUVECs).
In this study, the effects of baicalin on thrombin-induced cell injury in HUVECs were examined, and the underlying mechanisms were investigated.
2. Materials and Methods
Thrombin (T6884) was purchased from Sigma-Aldrich (St. Louis, MO, USA). Baicalin was purchased from Haotian Pharmaceutical Company (Chinese Drug Approval No. H20073931, 95% purity, Weifang, China) and dissolved in dimethyl sulfoxide. 3-(4,5-dimethylthiazol-2-yl)-2,5-diphenyltetrazolium bromide (MTT) was purchased from Amresco (OH, USA). Annexin V-FITC/PI Apoptosis Detection Kit was obtained from BD Pharmingen. Caspase-3 assay kit was purchased from Sigma-Aldrich (St. Louis, MO, USA). Trizol RNA-RNAiso Plus, Prime Script RT reagent kit with gDNA Eraser, and SYBR premix Ex Tap were purchased from TakaRa (Dalian, China). Antibodies against PAR-1, caspase-3, P65, p-P65, ERK1/2, p-ERK1/2, and GAPDH were obtained from Abcam (Cambridge, UK). Goat anti-rabbit IgG antibody was obtained from GenScript (Nanjing, China).
2.2. Cell Lines and Cell Culture
HUVECs were obtained from American Type Culture Collection (ATCC, Manassas, VA, USA) and maintained in RPMI-1640 (Corning) supplemented with 10% fetal bovine serum (FBS, Gibco), penicillin G (100 U/mL), and streptomycin (100 μg/mL) in a 5% CO2 incubator at 37°C. Cells of the 4-8 generation were used in all experiments. In experiments for thrombin stimulation, HUVECs were pretreated with baicalin at different concentrations (0 μM, 50 μM, 100 μM, and 150 μM) for 3 hours, followed by treatment with thrombin (5 U/mL) for additional 6 hours.
2.3. Cell Proliferation Assay
HUVECs were seeded in 96-well plates at a density of 1 × 104 cells per well and treated with baicalin and thrombin. The MTT solution was added to each well at a concentration of 5 mg/mL and the cells were cultured for additional 4 hours at 37°C. Supernatants were removed and replaced with 150 μL dimethyl sulfoxide (DMSO) into each well. Ten minutes later, the absorbance of each well was measured at 490 nm using a microplate reader.
2.4. Cell Apoptosis Assay
HUVECs were seeded in 6-well plates at a density of 2 × 105 cells per well and treated with baicalin and thrombin. Next, cells and supernatants were collected, washed with phosphate buffered solution (PBS), and resuspended in 100 μL1 × binding buffer. Then 5 μL of FITC-labelled Annexin V and PI were added and incubated at room temperature in the dark. After 15 minutes, 400 μL1 × binding buffer was added. Cell apoptosis was analyzed using flow cytometry.
2.5. Measurement of Caspase-3 Activity
HUVECs were treated with baicalin and thrombin. According to the manufacturer’s instructions, the activity of caspase-3 like protease in pyrolysis solution was evaluated by using colorimetric caspase-3 assay kit. In brief, the reaction mixture (total volume, 100 μL) including 30 μL of cell lysate and 10 μL of caspase-3 substrate acetyl–Asp–Glu–Val–Asp–p-nitroanilide (final concentration at 200μM) was used and determined on 96-well plate. The mixture was incubated for 90 minutes at 37°C and the absorbance was measured at 405 nm. The caspase-3 activity was expressed by value of OD405 relative to control.
2.6. RNA Extraction and Quantitative Real-Time Polymerase Chain Reaction
Total RNA was extracted purified using Trizol RNA-RNAiso Plus. Reverse transcription was performed to generate complementary DNA (cDNA) using Prime Script RT reagent kit with gDNA Eraser according to manufacturer’s protocol. The mRNA expression of PAR-1 was measured by quantitative real-time polymerase chain reaction using SYBR premix Ex Tap TM (TLiRNSEH PLUS). Predesigned primers were as follows: β-actin forward, 5′-TGACGTGGACATCCGCAAAG-3′; β-actin reverse, 5′-CTGGAAGGTGGACAGCGAGG-3′; PAR-1 forward, 5′-CACAAACGTCCTCCTGATTG-3′; PAR-1 reverse, 5′-ATGCTGCTGACACAGACACA-3′; β-actin was used as internal control. The relative mRNA expression of these genes was calculated using the 2 method.
2.7. Western Blotting
Cells were lysed with lysis buffer containing protease inhibitors and NP-40, and the protein concentration was quantified using Bicinchoninic acid (BCA) assay. Next, the protein samples (40 μg per lane) were subjected to SDS-PAGE and transferred to a polyvinylidene fluoride membrane. The membrane was blocked in 5％ nonfat milk at room temperature for an hour and then incubated with antibodies at 4°C overnight. The membrane was washed 3 times with PBS containing 0.5％ Tween-20 and incubated with corresponding horseradish peroxidase-conjugated secondary antibody for 2 hours. The blots were visualized using enhanced chemiluminescence (Perkin Elmer, Boston, MA, USA).
2.8. Statistical Analysis
All data are shown as the mean ± standard deviation (SD). Statistical differences between the groups were determined by repeated measurement analysis of variance tests. All statistical analyses were conducted using GraphPad Prism 5.0 (GraphPad Software Inc., San Diego, CA, USA). A value of P< 0.05 was considered statistically significant.
3.1. Effect of Baicalin on Thrombin-Induced Inhibition of Cell Survival
First, the effect of baicalin on thrombin-induced cell damage was evaluated in HUVECs. Cell viability was analyzed by MTT assay. HUVECs were pretreated with baicalin at different concentrations (0 μM, 50 μM, 100 μM, and 150 μM) for 3 hours, followed by treatment with thrombin (5 U/ml) for additional 6 hours. As shown in Figure 1(a), compared with control cells, cell viability was significantly decreased in HUVECs treated with thrombin. The inhibitory effect of thrombin on cell viability was partially abolished by pretreatment with baicalin in a dose-dependent manner.
3.2. Inhibitory Effect of Baicalin on Thrombin-Induced Cell Apoptosis
As MTT assay could not make a distinction between cells undergoing necrosis or apoptosis, flow cytometry was performed to determine cell apoptosis. As shown in Figures 1(b) and 1(c), compared with control cells, the percentage of apoptotic cells increased in HUVECs treated with thrombin. Pretreatment with baicalin decreased thrombin-induced cell apoptosis in a dose-dependent manner.
To verify the above results, the activity of caspase-3 was determined by using a caspase-3 assay kit, and the levels of caspase-3 and cleaved caspase-3 protein were examined by western blotting. As shown in Figure 1(d), compared with control cells, thrombin induced caspase-3 activation, which was inhibited by baicalin in a dose-dependent manner. As shown in Figures 1(e) and 1(f), western blot analysis revealed a higher level of cleaved caspase-3 in thrombin treated cells than control cells. Accordingly, baicalin decreased the level of cleaved caspase-3.
3.3. Inhibitory Effect of Baicalin on Thrombin-Induced NF-κB Activation
NF-κB was activated upon thrombin stimulation and contributed to cell injury in previous study. In the present study, we evaluated NF-κB activation by detection of P65 phosphorylation. The expression of NF-κB (P65) and p-P65 was determined by western blotting. As shown in Figures 2(a) and 2(b), the expression of p-P65 was significantly increased in HUVECs treated with thrombin compared with control cells, which was attenuated by baicalin in a dose-dependent manner.
3.4. Inhibitory Effect of Baicalin on Thrombin-Induced PAR-1 Expression
PAR-1 was shown to participate in the processes of cell apoptosis. Thus, we examined the effect of baicalin on thrombin induced PAR-1 expression. The expression of PAR-1 in mRNA and protein levels was determined by RT-PCR and western blotting, respectively. As shown in Figure 3, the expression of PAR-1 was significantly increased in mRNA and protein levels after thrombin treatment, which was partly inhibited by baicalin in a dose-dependent manner.
3.5. Baicalin Decreased Thrombin-Induced PAR-1 Expression through Inhibition of ERK1/2 Phosphorylation
To investigate the mechanism of baicalin inhibiting PAR-1 expression, we detected the phosphorylation of ERK1/2. HUVECs were pretreated with U0126 (10 μM) for 3 hours before exposure to thrombin (5 U/ml). As shown in Figure 4(a), thrombin exposure in HUVEC induced a rapid ERK1/2 phosphorylation, which was partly abrogated by pretreatment of U0126 (10 μM), a selective inhibitor of MAP kinase. Similarly, pretreatment with baicalin (50 μM) also partly inhibited thrombin-induced ERK1/2 phosphorylation as shown in Figure 4(b). Both U0126 and baicalin decreased thrombin-induced PAR-1 expression.
In this study, we demonstrated that baicalin significantly inhibited thrombin-induced upregulation of cell apoptosis in HUVECs. The major mechanisms included inhibition of PAR-1 expression and inhibition of MAP kinase, NF-κB, and caspase-3 activation.
Endothelial cells apoptosis occurs throughout the early stages of atherosclerosis and plays important roles in plaque regression and plaque instability [18, 19]. Apoptosis, or programed cell death, is a serious form of endothelial cells injury and fundamental to physiologic processes . The signaling pathways leading to apoptosis can generally be divided into the extrinsic (surface receptor-mediated) and intrinsic (mitochondrial dependent) pathways . Apoptotic pathways can be modulated by various inflammatory molecules and elucidation of these mechanisms may lead to novel therapeutic interventions that inhibit key steps in the apoptosis pathways. Apoptosis is tightly regulated and primarily carried out by aspartate-specific cysteine proteases termed “caspases”. As is known to all, caspase-3 cleavage is the main hallmark of apoptosis . In this study, compared with cells in the control group, the percentage of apoptotic cells increased in HUVECs treated with thrombin, and pretreatment with baicalin decreased thrombin-induced cell apoptosis in a dose-dependent manner. We found that baicalin inhibited the thrombin-induced caspase-3 activation in a dose-dependent manner.
The expression of thrombin was elevated in patients with ischemic cerebrovascular disease (CVD) in the previous reports [14, 23]. Protease activated receptors, which are abundantly expressed in all arterial vessel wall, are a family of G-protein coupled receptors comprising four members (i.e., PAR-1, PAR-2, PAR-3, and PAR-4) . However, thrombin interacts with PAR-1 to participate a number of biological processes, such as inhibition of cell proliferation, induction of cell apoptosis, activation of inflammation and upregulation of adhesion molecules and matrix metalloproteinase (MMP) [25, 26]. Previous studies reported that the expression of PAR-1 was upregulated after thrombin stimulation in rodent models . PAR-1 activation by thrombin has been found to activate or inhibit apoptosis in neuronal cells, astrocytes, endothelial cells, epithelial cells, fibroblasts, and tumor cells in a dose-dependent fashion [28–30]. In addition, it has been found that PAR-1 activation can increase epithelial cell apoptosis and intestinal permeability in a caspase-3 dependent manner . Our results showed that PAR-1 was dramatically upregulated after thrombin stimulation in HUVECs, while baicalin inhibited the expression of PAR-1 in a dose-dependent manner.
Nuclear factor (NF)-κB signaling was associated with the transcriptional regulation of various genes involved in inflammatory responses, cell growth, survival, and apoptosis [31, 32]. In unstimulated cells, NF-κB binds to inhibitory molecule IκB which retains NF-κB in an unstimulated state and prevents its migration to nucleus. Upon stimulated, IκB is degraded, releasing NF-κB that translocates to the nucleus and promotes target genes transcription . It can be found that NF-κB can be activated upon thrombin stimulation and caused cell injury [7, 34]. The importance of NF-κB signaling in regulating the apoptotic program has been demonstrated in various cells . It can be demonstrated that NF-κB signaling is crucial in preventing heat stress-induced apoptosis of HUVECs . It was also found that activated HUVECs are involved in atherosclerosis through the activation of NF-κB and release inflammatory factors . It has been suggested that PAR-1 causes apoptosis of cells to be regulated by activation of NF-κB [37, 38]. Baicalin attenuated thrombin-induced upregulation of NF-κB in SH-SY5Y cells . Consistent with previous studies, we demonstrated that baicalin inhibited thrombin-induced activation of NF-κB in a dose-dependent manner in HUVECs.
Baicalin is a kind of Chinese traditional medicine, which has multiple potential biological functions anti-inflammatory and antiapoptosis [39, 40]. However, the biotransformation of baicalin is poorly understood. It is due in part to difficulties that have been encountered in obtaining enough amounts to identify the structure of the metabolites and study the bioactivities of them . To explore the mechanism of baicalin in inducing thrombin-induced cell apoptosis in HUVECs, we studied the effect of baicalin on the PAR-1 expression and NF-κB activation. In the present study, we found that thrombin upregulated PAR-1 expression and then activated NF-κB pathway, which caused cell apoptosis in HUVECs. Baicalin protected against thrombin-induced cell injury by inhibiting the expression of PAR-1 and NF-κB activation.
Increasing evidence suggests that activation of the ERK signaling pathway is also involved in inflammation and apoptosis [42, 43]. Thrombin-mediated PAR-1 gene expression in endothelial cells requires the heterotrimeric Gi-activated Ras/MAPK signaling pathway . Besides, ERK signaling pathway plays a key role in baicalin protection against oxygen-glucose deprivation induced rat brain microvascular endothelial cells injury and acetaminophen-induced liver injury [45, 46]. To get more insight into the mechanism of baicalin on thrombin-induced cell injury, we examined the effect of baicalin on ERK1/2 activation. Our results showed that thrombin-induced PAR-1 expression was accompanied with concomitant activation of ERK1/2. U0126, a specific inhibitor of ERK1/2, prevented thrombin-induced ERK1/2 activation and partly inhibited thrombin-induced PAR-1 expression. These results suggested that thrombin-induced PAR-1 expression is at least partly mediated by ERK1/2 activation. Further experiments showed that baicalin had a similar effect as U0126. Pretreatment with baicalin partly inhibited thrombin-induced ERK1/2 activation and PAR-1 expression. We proposed that baicalin can inhibit PAR-1 expression by inhibiting ERK pathway. In future, further studies are required to investigate the mechanism by which baicalin prevents ERK1/2 activation.
In conclusion, our study showed that baicalin has protective effects on thrombin-induced cell injury in HUVECs possibly through inhibition of PAR-1 expression and its downstream NF-κB activation, raising the possibility of use of baicalin as a drug for the prevention and treatment of atherosclerosis. Baicalin could inhibit thrombin-induced PAR-1 expression, which was mediated by ERK1/2 activation.
The data used to support the findings of this study are included within the article.
Conflicts of Interest
The authors declare that they have no conflicts of interest.
This work is supported by the Shandong Province Key Research and Development Projects (Grant no. 2016GSF201050), National Natural Science Fund Program of China (Grant no. 81072916), and Basic Scientific Research Business Expenses Funded Project of Shandong University (Grant no. 2016JC026).
- J. Kalz, C. H. Ten, and H. M. Spronk, “Thrombin generation and atherosclerosis,” Journal of Thrombosis and Thrombolysis, vol. 37, no. 1, pp. 45–55, 2014.
- J. Yong, D. Lin, and X. R. Tan, “Primary prevention of cardiovascular disease in older adults in China,” World Journal of Clinical Cases, vol. 5, no. 9, pp. 349–359, 2017.
- J. I. Borissoff, H. M. H. Spronk, S. Heeneman, and H. T. Cate, “Is thrombin a key player in the "coagulation-atherogenesis" maze?” Cardiovascular Research, vol. 82, no. 3, pp. 392–403, 2009.
- J. I. Borissoff, S. Heeneman, E. Kilinç et al., “Early atherosclerosis exhibits an enhanced procoagulant state,” Circulation, vol. 122, no. 8, pp. 821–830, 2010.
- J. I. Borissoff, H. M. H. Spronk, and H. T. Cate, “The hemostatic system as a modulator of atherosclerosis,” The New England Journal of Medicine, vol. 364, no. 18, pp. 1746–1760, 2011.
- D. Fritze, W. Zhang, J. Li, B. Chai, and M. W. Mulholland, “TNF-α causes thrombin-dependent vagal neuron apoptosis in inflammatory bowel disease,” Journal of Gastrointestinal Surgery, vol. 18, no. 9, pp. 1632–1641, 2014.
- C. Cowan, C. K. Muraleedharan, J. J. O'Donnell et al., “MicroRNA-146 inhibits thrombin-induced NF-κB activation and subsequent inflammatory responses in human retinal endothelial cells,” Investigative Ophthalmology & Visual Science, vol. 55, no. 8, pp. 4944–4951, 2014.
- E. Middleton and G. Drzewiecki, “Flavonoid inhibition of human basophil histamine release stimulated by various agents,” Biochemical Pharmacology, vol. 33, no. 21, pp. 3333–3338, 1984.
- N. Mukaida, “Interleukin-8: an expanding universe beyond neutrophil chemotaxis and activation,” International Journal of Hematology, vol. 72, pp. 391–398, 2000.
- J. Sun, L. L. Li, J. F. Wu et al., “Effects of baicalin on airway remodeling in asthmatic mice,” Planta Medica, vol. 79, no. 3-4, pp. 199–206, 2013.
- M. Kubo, H. Matsuda, M. Tanaka et al., “Studies on Scutellariae radix. VII. Anti-arthritic and anti-inflammatory actions of methanolic extract and flavonoid components from Scutellariae radix,” Chemical Pharmaceutical Bulletin (Tokyo), vol. 32, no. 7, pp. 2724–2729, 1984.
- D. Kim, E. Son, M. Kim et al., “Antiallergic herbal composition from scutellaria baicalensis and phyllostachys edulis,” Planta Medica, vol. 76, no. 7, pp. 678–682, 2010.
- X. N. Ju, W. N. Mu, Y. T. Liu et al., “Baicalin protects against thrombin induced cell injury in SH-SY5Y cells,” International Journal of Clinical & Experimental Pathology, vol. 8, no. 11, p. 14021, 2015.
- Q. Zhou, C. Duan, Q. Jia, P. Liu, and L. Li, “Baicalin attenuates focal cerebral ischemic reperfusion injury by inhibition of protease-activated receptor-1 and apoptosis,” Chinese Journal of Integrative Medicine, vol. 20, no. 2, pp. 116–122, 2014.
- B. Wang, P.-P. Liao, L.-H. Liu, X. Fang, W. Li, and S.-M. Guan, “Baicalin and geniposide inhibit the development of atherosclerosis by increasing Wnt1 and inhibiting dickkopf-related protein-1 expression,” Journal of Geriatric Cardiology, vol. 13, no. 10, pp. 846–854, 2016.
- Y. Zhang, P. Liao, M. Zhu et al., “Baicalin attenuates cardiac dysfunction and myocardial remodeling in a chronic pressure-overload mice model,” Cellular Physiology and Biochemistry, vol. 41, no. 3, pp. 849–864, 2017.
- P. Liao, L. Liu, B. Wang, W. Li, X. Fang, and S. Guan, “Baicalin and geniposide attenuate atherosclerosis involving lipids regulation and immunoregulation in ApoE-/- mice,” European Journal of Pharmacology, vol. 740, pp. 488–495, 2014.
- M. A. Gimbrone and G. García-Cardeña, “Endothelial cell dysfunction and the pathobiology of atherosclerosis,” Circulation Research, vol. 118, no. 4, pp. 620–636, 2016.
- J. E. Deanfield, J. P. Halcox, and T. J. Rabelink, “Endothelial function and dysfunction: testing and clinical relevance,” Circulation, vol. 115, no. 10, pp. 1285–1295, 2007.
- L. Quan, Z. Jian, Z. Ping, and L. Weiming, “Proteinase-activated receptor-1 mediates allogeneic CD8+ T cell-induced apoptosis of vascular endothelial cells,” Medical Oncology, vol. 26, no. 4, pp. 379–385, 2009.
- K. M. Hajra and J. R. Liu, “Apoptosome dysfunction in human cancer,” Apoptosis, vol. 9, no. 6, pp. 691–704, 2004.
- A. N. Flynn and A. G. Buret, “Proteinase-activated receptor 1 (PAR-1) and cell apoptosis,” Apoptosis, vol. 9, no. 6, pp. 729–737, 2004.
- Y. Hua, J. Wu, R. F. Keep et al., “Thrombin exacerbates brain edema in focal cerebral ischemia,” Acta Neurochirurgica, vol. 86, no. 86, pp. 163–166, 2003.
- C. Yang, L. Hsiao, C. Yang, and C. Lin, “Thrombin Enhanced Matrix Metalloproteinase-9 Expression and Migration of SK-N-SH Cells via PAR-1, c-Src, PYK2, EGFR, Erk1/2 and AP-1,” Molecular Neurobiology, vol. 54, no. 5, pp. 3476–3491, 2017.
- J. C. Reséndiz, M. H. Kroll, and R. Lassila, “Protease-activated receptor-induced Akt activation - regulation and possible function,” Journal of Thrombosis and Haemostasis, vol. 5, no. 12, pp. 2484–2493, 2007.
- R. Ramachandran and M. D. Hollenberg, “Proteinases and signalling: pathophysiological and therapeutic implications via PARs and more,” British Journal of Pharmacology, vol. 153, supplement 1, pp. S263–S282, 2008.
- P. Rajput, P. Lyden, B. Chen et al., “Protease activated receptor-1 mediates cytotoxicity during ischemia using in vivo and in vitro models,” Neuroscience, vol. 281, pp. 229–240, 2014.
- L. O. Mosnier and J. H. Griffin, “Inhibition of staurosporine-induced apoptosis of endothelial cells by activated protein C requires protease-activated receptor-1 and endothelial cell protein C receptor,” Biochemical Journal, vol. 373, no. 1, pp. 65–70, 2003.
- F. M. Donovan, C. J. Pike, C. W. Cotman, and D. D. Cunningham, “Thrombin induces apoptosis in cultured neurons and astrocytes via a pathway requiring tyrosine kinase and RhoA activities,” The Journal of Neuroscience, vol. 17, no. 14, pp. 5316–5326, 1997.
- A. C. Chin, N. Vergnolle, W. K. MacNaughton, J. L. Wallace, M. D. Hollenberg, and A. G. Buret, “Proteinase-activated receptor 1 activation induces epithelial apoptosis and increases intestinal permeability,” Proceedings of the National Acadamy of Sciences of the United States of America, vol. 100, no. 19, pp. 11104–11109, 2011.
- A. S. Baldwin, “Control of oncogenesis and cancer therapy resistance by the transcription factor NF-κB,” The Journal of Clinical Investigation, vol. 107, no. 3, pp. 241–246, 2001.
- H. L. Pahl, “Activators and target genes of Rel/ NF-κB transcription factors,” Oncogene, vol. 18, no. 49, pp. 6853–6866, 1999.
- S. Mitchell, J. Vargas, and A. Hoffmann, “Signaling via the NF-κB system,” Wiley Interdisciplinary Reviews Systems Biology & Medicine, vol. 8, no. 3, pp. 227–241, 2016.
- D. Fritze, W. Zhang, J. Y. Li et al., “TNFα causes thrombin-dependent vagal neuron apoptosis in inflammatory bowel disease,” Journal of Gastrointestinal Surgery, vol. 18, no. 9, pp. 1632–1641, 2014.
- Y. Liu, G. Zhou, Z. Wang et al., “NF-κB signaling is essential for resistance to heat stress-induced early stage apoptosis in human umbilical vein endothelial cells,” Scientific Reports, vol. 5, no. 1, p. 13547, 2015.
- T. Collins and M. I. Cybulsky, “NF-κB: pivotal mediator or innocent bystander in atherogenesis?” The Journal of Clinical Investigation, vol. 107, no. 3, pp. 255–264, 2001.
- S. Zhang, Y. Liu, Z. Wang et al., “PAR1-mediated c-Jun activation promotes heat stress-induced early stage apoptosis of human umbilical vein endothelial cells,” Molecular Medicine Reports, vol. 15, no. 5, pp. 2595–2603, 2017.
- T. Ray and A. Pal, “PAR-1 mediated apoptosis of breast cancer cells by V. cholerae hemagglutinin protease,” Apoptosis, vol. 21, no. 5, pp. 609–620, 2016.
- W. Yang, H. Li, X. Cong et al., “Baicalin attenuates lipopolysaccharide induced inflammation and apoptosis of cow mammary epithelial cells by regulating NF-κB and HSP72,” International Immunopharmacology, vol. 40, pp. 139–145, 2016.
- J. Liu, Y. Wei, Q. Luo et al., “Baicalin attenuates inflammation in mice with OVA-induced asthma by inhibiting NF-κB and suppressing CCR7/CCL19/CCL21,” International Journal of Molecular Medicine, vol. 38, no. 5, pp. 1541–1548, 2016.
- Y. Wang, Y. Jia, X. Yang, B. Liang, H. Gao, and T. Yang, “A potential role of Baicalin to inhibit apoptosis and protect against acute liver and kidney injury in rat preeclampsia model,” Biomedicine & Pharmacotherapy, vol. 108, pp. 1546–1552, 2018.
- G. Nowak and Y. Nowak, “Protein kinase C-αand ERK1/2 mediate mitochondrial dysfunction, decreases inactive Na+ transport, and cisplatin induced apoptosis in renal cells,” Journal of Biological Chemistry, vol. 277, no. 45, pp. 43377–43388, 2002.
- S.-K. Jo, W. Y. Cho, S. A. Sung et al., “MEK inhibitor, U0126, attenuates cisplatin-induced renal injury by decreasing inflammation and apoptosis,” Kidney International, vol. 67, no. 2, pp. 458–466, 2005.
- C. A. Ellis, A. B. Malik, A. Gilchrist et al., “Thrombin induces proteinase-activated receptor-1 gene expression in endothelial cells via activation of Gi-linked Ras/mitogen-activated protein kinase pathway,” The Journal of Biological Chemistry, vol. 274, no. 19, pp. 13718–13727, 1999.
- P. Zhang, J. Hou, J. Fu, D. Li, C. Zhang, and J. Liu, “Baicalin protects rat brain microvascular endothelial cells injured by oxygen-glucose deprivation via anti-inflammation,” Brain Research Bulletin, vol. 97, pp. 8–15, 2013.
- C. Liao, Y. Day, H. Lee, J. Liou, A. Chou, and F. Liu, “ERK signaling pathway plays a key role in baicalin protection against acetaminophen-induced liver injury,” American Journal of Chinese Medicine, vol. 45, no. 01, pp. 105–121, 2017.
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