Oleanolic acid protects against oxidative stress‑induced human umbilical vein endothelial cell injury by activating AKT/eNOS signaling.

Oxidative injury of vascular endothelial cells in the initial event of atherosclerosis (AS) in diabetes was assessed in the present study. The antioxidant effect of oleanolic acid (OA) has attracted much attention. In the present study the potential effects of OA on human umbilical vein endothelial cells (HUVECs) were investigated. Cell viability was examined using the CCK‑8 assay. The activity of oxidative stress parameters was determined using commercial kits. Flow cytometry analysis was performed to detect the level of reactive oxygen species (ROS), mitochondrial membrane potential (MMP) and cell apoptosis. The expression levels of target genes and proteins were examined by reverse transcription‑quantitative polymerase chain reaction (RT‑qPCR) and western blot analysis. It was indicated that cell viability that was suppressed by high glucose was increased by the pretreatment of OA, and nitric oxide (NO) generation, the activities of superoxide dismutase (SOD) and catalase (CAT) were recovered by OA. By contrast, it was observed that OA decreased the MDA content. Notably, the pretreatment of OA alleviated mitochondria damage by reducing the level of ROS and maintaining MMP. In addition, apoptosis that was caused by high glucose was reduced by OA. Pro‑apoptotic genes (caspase‑3, Fas, Fasl) and anti‑apoptotic gene (Bcl‑2) expression levels were decreased and increased in the OA groups, respectively. Furthermore, the activity of AKT/endothelial nitric oxide synthase (eNOS) signaling was elevated by OA. Taken together, it was suggested that OA could protect against oxidative stress‑induced apoptosis of HUVECs, which was associated with AKT/eNOS signaling pathway.

Introduction

Atherosclerosis (AS) is a common complication of diabetes. Arteriosclerosis in diabetic patients has higher mortality than that among the non-diabetic (1,2). Hyperglycemia is a primary phenotype of diabetic patients (3). Vascular endothelial cells are critical targets of hyperglycemia injury in diabetes mellitus (4). The injury of vascular endothelial cells is the initial event of AS (5). Moreover, oxidative stress caused by hyperglycemia is a main inducement of vascular endothelial cells injury (6), which is resulted from the imbalance between production and removal of reactive oxygen species (ROS) (7). In normal circumstances, intracellular antioxidant systems, for instance, superoxide dismutase (SOD) and catalase (CAT), maintain the cell redox self-steady state (8). Nevertheless, ROS accumulation will induce lipid peroxidation, resulting in the production of MDA (9,10). Moreover, excessive exposure of ROS can lead to the dysfunction of the vascular endothelial cells (11). Vascular endothelium, a complex endocrine organ (12), could secrete cytoactive factors in response to the change of signals and stress (13). Nitric oxide (NO) plays a critical role in maintaining the vasoconstrictor function, which is a primary endogenous vascular diastolic factor (14). Additionally, NO is helpful to the inhibition of the production of oxygen free radicals (15). It has been documented that oxidative stress and the production or activation of NO were essential for the AS (8).

Furthermore, studies have pointed out that cell apoptosis was closely linked to the ROS accumulation (3,16,17). Importantly, high glucose can promote apoptosis of human umbilical vein endothelial cells (HUVECs) (18). Hence, alleviation of high glucose-induced oxidative stress and apoptosis of endothelial cells may play an important role in the prevention and treatment of AS and other diabetic macrovascular diseases. The PI3K/AKT signaling functions critically in cellular death progression (19). It is well known that the survival of endothelial cells could be maintained by AKT. Moreover, AKT could activate the expression of endothelial nitric oxide synthase (eNOS) (20), which is responsible for the production of NO (21). Therefore, in this study, we paid close attention to the AKT/eNOS signaling for its protective role in endothelial cells.

As previously described (22), oleanolic acid (OA), which is a pentacyclic triterpenoid compound, is widespread in plants. OA has several pharmacological activities. The antitumor effect of OA has been noted previously (23–26). Studies have also reported that OA could exert anti-oxidative effect (27,28). OA is believed to be able to treat diabetes (29,30), and it is reported to be related to arteriosclerosis (31). Thus, it is of research significance to assess the effects of OA on high-glucose induced oxidative stress in HUVECs.

In the present study, we sought to evaluate the effects of OA in HUVECs cultivated in vitro via detecting the oxidative response and apoptosis of HUVECs. The mechanism action of OA was as well investigated. Our research provides reference for developing candidate agent in the treatment of AS in diabetics.

Materials and methods

Cell culture and treatment

HUVECs (ATCC, USA) were maintained in Dulbecco's modified Eagle's medium (DMEM) (HyClone; GE Healthcare Life Sciences, Logan, UT, USA) that contained 10% FBS (Gibco; Thermo Fisher Scientific, Inc., Waltham, MA, USA) and penicillin/streptomycin (Beijing Solarbio Science & Technology Co., Ltd., Beijing, China) at 37°C in an incubator with 5% CO2. The normal blood glucose level ranged from 3.9 and 5.5 mM (32) in non-diabetics. Blood sugar levels increased more than normal range may be an indicator of diabetes. According to some researches on hyperglycemia injury model in vitro (33,34), HUVECs were respectively treated with glucose at 5 and 33 mM for the control and injury model for 48 h. The incubation concentration of OA was determined in reference to a previous study (35). The research groups in this study were classified as follow: Blank group (blank): no glucose treatment; control group (Con): 5 mM glucose treatment; High glucose model group (GC): 33 mM glucose (Sangon Biotech Co., Ltd., Shanghai, China) treatment; positive control group (OA-H/Con): 40 mM OA (purity >98%; Beijing Solarbio Science & Technology Co., Ltd.) (dissolved in ethanol) for incubation for 24 h prior to 5 mM glucose treatment; low OA treatment group (OA-L/GC): Cells were treated with 20 mM OA at 37°C for 24 h prior to 33 mM glucose treatment; high OA treatment group (OA-H/GC): Cells were treated with 40 mM OA at 37°C for 24 h prior to 33 mM glucose treatment.

Cell viability assay

The cell survival rate was examined using Cell Counting Kit-8 (CCK-8; Beyotime Institute of Biotechnology, Haimen, China) assay, according to the manufacturer's protocols. To explain further, 1×104/each well were seeded into a 96-well plate and incubated at 37°C for 24 h. CCK-8 (10 µl/well) was added into the 96-well plate, and then the cells were incubated at 37°C for 4 h. Absorbance at 450 nm was detected using a microplate reader (PerkinElmer, Inc., Waltham, MA, USA).

ROS measurement

Intracellular ROS level was detected using fluorescent probe DCFH-DA probe (Sigma-Aldrich; Merck KGaA, Darmstadt, Germany). Cells were collected and washed by PBS. Next, the cells were maintained with 10 µM DCHF-DA in darkness at 37°C for 30 min. Flow cytometry analysis was carried out to examine the fluorescence signals corresponding to DCHF-DA on flow cytometer (BD Biosciences, Franklin Lakes, NJ, USA) with Cell Quest software version 5.1 (BD Biosciences). At least 10,000 events were analyzed in each examination.

Detection for mitochondrial transmembrane potential (MMP)

The Rho 123 accumulation was determined by flow cytometry analysis as previously described (36). Following the treatment above, the cells in 24-well plates (2×105 cells/well) were incubated with 50 mM Rho 123 (Sigma-Aldrich; Merck KGaA) at 37°C for 30 min. The reaction was terminated at 5 min of incubation on ice. Subsequently, the fluorescent of Rho 123 was detected by FACS Calibur flow cytometer (BD Biosciences). Cell Quest software version 5.1 (BD Biosciences) was used to perform the analysis.

Detection of apoptosis

Annexin V-FITC (Sigma-Aldrich; Merck KGaA)/PI (Sigma-Aldrich; Merck KGaA) double-staining for apoptosis analysis was used to determine the aopotosis by flow cytometry analysis. To be more specific, the cells in 6-well plate at a density of 2×106/well were treated as above. Subsequently, the cells were incubated with 5 ul Annexin V-FITC for10 min at room temperature and with 5 µl PI at room temperature for 15 min in the darkness. FACS Calibur flow cytometer (BD Biosciences) and Cell Quest software version 5.1 were used to count the apoptotic cells.

Measurement of NO level

The generation of NO was examined with commercial Nitrate/Nitrite Fluorometric Assay kit (Cayman Chemical Company, Ann Arbor, MI, USA) through nitrate reductase method via its breakdown products, Nitrate/Nitrite, After conducting treatment as designed, the determination was performed following manufacturer's protocols.

Measurement of SOD, CAT, and MDA level

Cells (1×104/well) were seeded into a 96-well plate and incubated at 37°C for 24 h. Then, the cells were centrifuged at 200 g for 5 min at 4°C. After being washed with PBS, the cells were resuspended and collected for the detection of the enzymes activities. The cellular SOD and CAT enzyme were determined using corresponding kits (Beijing Solarbio Science & Technology Co., Ltd.), according to the protocols. The MDA content was detected with thiobarbituric acid substance provided by Malondialdehyde Assay Kit (Beyotime, China).

Reverse transcription-quantitative polymerase chain reaction (RT-qPCR) analysis

Total RNA was exacted using RNAiso Plus (Invitrogen; Thermo Fisher Scientific, Inc.). M-MLV (Promega Corporation, Madison, WI, USA) and oligo (dT) primers (Takara Bio, Inc., Otsu, Japan) were used to synthesis cDNA from RNA (1 µg). The temperature and incubation protocol was set at 25°C for 10 min, at 42°C for 50 min, at 70°C for 10 min. Amplification of the related genes was conducted using LightCycler® 480 SYBR-Green I Master (Roche Diagnostics, Indianapolis, IN, USA). The thermal cycle conditions was as follows: At 95°C, 4 min; at 35 cycles of 95°C, 15 Sec; at 60°C, 45 Sec; at 72°C, 7 min. The expression of target genes was normalized using the expression levels of GAPDH according to 2−ΔΔCq method (37). The primers used were as follows: Fas forward 5′-GTGCTTTGCTTAGGGTTCCC-3′, Fas reverse 5′-AACTTGCACTTCTGGCCATG-3′; Fasl forward 5′-GTCCAACTCAAGGTCCATGC-3′, Fasl reverse 5′-TTGTTGCAAGATTGACCCCG-3′; Bax forward 5′-GTGCCGGAACTGATCAGAAC-3′, Bax reverse 5′-CCAAAGTAGGAGAGGAGGCC-3′; Bcl-2 forward 5′-GCCTTCTTTGAGTTCGGTGG-3′, Bcl-2 reverse 5′-GAAATCAAACAGAGGCCGCA-3′; GAPDH forward: 5′-CACAGTCCATGCCATCACTG-3′; GAPDH reverse: 5′-ATCTCGCTCCTGGAAGATGG-3′;

Western blot analysis

Cells were lysed using 200 µl lysis buffer NP40 (Beyotime Institute of Biotechnology). The concentration of the samples was determined by BCA protein quantitative kit (Bio-Rad Laboratories, Inc., Hercules, CA, USA). Proteins were separated using 10% SDS-PAGE gels and transferred onto a PVDF membrane (EMD Millipore, Billerica, MA, USA). After being blocked with 5% non-skimmed milk at room temperature for 2 h, the membrane was incubated with primary antibodies as listed: cleaved caspase-3 (ab32042, 1:500; Abcam, Cambridge, UK), Fas (ab82419, 1:1,000), Fasl (ab15285, 1 ug/ml), Bax (ab32503,1:2,000), Bcl-2 (ab32124, 1:1,000), p-AKT (ab812831:5,000), AKT 1/2 (ab182729, 1:5,000), p-eNOS (ab184154, 1:1,000), eNOS (ab76198, 1:1,000), and GAPDH (ab8245, 1:5,000), at 4°C overnight. Then, horseradish peroxidase-conjugated secondary antibody (ab6721, 1:4,000) was added and maintained at room temperature for 1 h. The blot bands were developed using BeyoECL Star (Beyotime Institute of Biotechnology). The gray density was calculated with Quantity One software version 4.6 (Bio-Rad Laboratories, Inc.).

Statistical analysis

Statistical analysis was calculated using GraphPad Prism software 6.0 (GraphPad Software, Inc., La Jolla, CA, USA). One-way ANOVA following Tukey's post hoc test was used to compare the difference between groups. The results were shown as means ± standard deviation. P<0.05 was considered to indicate a statistically significant difference.

Results

OA protected against high-glucose-induced injury in HUVECs

We first determined the effect of OA on cell viability of HUVECs. The CCK-8 test showed that the cell survival rate of HUVECs decreased obviously in the GC group in comparison to that in the control group, and that the pretreatment of OA improved the cell survival rate in a dose-dependent manner (Fig. 1A). Moreover, the nitric oxide (NO) generation was rescued by the pretreatment of OA (Fig. 1B). We also found that as an indicator of lipid peroxidation, the production of MDA caused by high glucose treatment was inhibited by the pretreatment of OA (Fig. 1C). Similarly, the activities of SOD and CAT were recovered in the pretreatment groups (Fig. 1D and E).

Figure 1.

OA protected against high-glucose-induced injury in HUVECs. (A) Cell viability of HUVECs was detected by CCK-8 assay when the cells were treated with high glucose and/or OA. (B-E) Detection of (B) NO content, (C) MDA level, (D) SOD activity and (E) CAT by available commercial kit when the cells were treated with high glucose and/or OA. Blank group (Blank), cuntreated cells; control group (5 mM) (Con/Control), cells were treated with 5 mM glucose; high glucose (33 mM) model group (GC), cells were treated with 33 mM glucose; positive control group (OA-H/Con), cells were treated with 5 mM glucose and 40 µM OA; low OA (20 µM) treatment group (OA-L/GC), cells were treated with 33 mM glucose and 20 µM OA; high OA (40 µM) treatment group (OA-H/GC), cells were treated with 33 mM glucose and 40 µM OA. **P<0.01, #P<0.01 and ^P<0.05 as indicated. OA, oleanolic acid; HUVECs; human umbilical vein endothelial cells; SOD, superoxide dismutase; CAT, catalase.

OA depressed the ROS production and mitochondrial membrane potential (MMP) loss in HUVECs

The increased ROS level is one of the sources causing mitochondria damage (38). The loss of MMP is an early hallmark event of mitochondria damage leading to apoptosis (39). Thus, the ROS production and the MMP of HUVECs were measured by flow cytometry analysis. Results showed that the ROS production was triggered by high glucose treatment. Noticeably, the ROS level was lower in the OA pretreatment groups than that in the GC group (Fig. 2A and B). Meanwhile, the loss of MMP caused by high glucose was recovered by the pretreatment of OA (Fig. 2C and D).

Figure 2.

OA prevented oxidative stress in HUVECs. (A and B) Flow cytometry assay for detection of cellular ROS analysis using DCFH-DA dye. (C and D) Flow cytometry analysis for detection of MMP using Rho123. Blank group (Blank), cuntreated cells; control group (5 mM) (Con/Control), cells were treated with 5 mM glucose; high glucose (33 mM) model group (GC), cells were treated with 33 mM glucose; positive control group (OA-H/Con), cells were treated with 5 mM glucose and 40 µM OA; low OA (20 µM) treatment group (OA-L/GC), cells were treated with 33 mM glucose and 20 µM OA; high OA (40 µM) treatment group (OA-H/GC), cells were treated with 33 mM glucose and 40 µM OA. **P<0.01, #P<0.05, ##P<0.01 and ^P<0.05 as indicated. OA, oleanolic acid; HUVECs; human umbilical vein endothelial cells; ROS, reactive oxygen species; MMP, mitochondrial transmembrane potential.

OA inhibited apoptosis caused by oxidative stress in HUVECs

ROS accumulation and the loss of MMP were both considered to be closely associated with apoptosis (40). Therefore, we further detected the apoptosis of HUVECs using flow cytometry analysis. The results indicated that the apoptosis of HUVECs induced by high glucose was apparently inhibited in the OA pretreatment groups (Fig. 3A and B). Moreover, the RT-qPCR and western blot assays showed that the expressions of pro-apoptotic genes including caspase-3, Fas, Fasl and Bax were lower in the OA pretreatment groups than those in the model group. By contrast, the expression of Bcl-2 was decreased in the model group but increased by the pretreatment of OA (Fig. 4C-E).

Figure 3.

OA decreased apoptosis of HUVECs. (A) Flow cytometry analysis for detection of cell apoptosis using Annexin V-FITC/PI staining. (B) Relative quantitative analysis of caspase-3, Fas, Fasl, Bax, and Bcl-2 by RT-qPCR. (C and D) Western blot analysis for caspase-3, Fas, Fasl, Bax, and Bcl-2. GAPDH was assessed as sample loading control. Blank group (Blank), cuntreated cells; control group (5 mM) (Con/Control), cells were treated with 5 mM glucose; high glucose (33 mM) model group (GC), cells were treated with 33 mM glucose; positive control group (OA-H/Con), cells were treated with 5 mM glucose and 40 µM OA; low OA (20 µM) treatment group (OA-L/GC), cells were treated with 33 mM glucose and 20 µM OA; high OA (40 µM) treatment group (OA-H/GC), cells were treated with 33 mM glucose and 40 µM OA. *P<0.05, **P<0.01, #P<0.05, ##P<0.01 and ^P<0.05 as indicated. OA, oleanolic acid; HUVECs; human umbilical vein endothelial cells; FITC, fluorescein isothiocyanate; PI, propidium iodide; RT-qPCR, reverse transcription-quantitative polymerase chain reaction.

Figure 4.

OA enhanced the activity of AKT/eNOS. (A and B) Western blot analysis for p-AKT and AKT. (C and D) Western blot analysis for the expression of p-eNOS and NOS. Blank group (Blank), cuntreated cells; control group (5 mM) (Con/Control), cells were treated with 5 mM glucose; high glucose (33 mM) model group (GC), cells were treated with 33 mM glucose; positive control group (OA-H/Con), cells were treated with 5 mM glucose and 40 µM OA; low OA (20 µM) treatment group (OA-L/GC), cells were treated with 33 mM glucose and 20 µM OA; high OA (40 µM) treatment group (OA-H/GC), cells were treated with 33 mM glucose and 40 µM OA. **P<0.01, #P<0.05 and ^P<0.05 as indicated. OA, oleanolic acid; eNOS, endothelial nitric oxide synthase.

OA enhanced the activity of AKT/eNOS signaling

To study the underlying mechanisms, the activity of AKT/eNOS signals was determined by Western blot. Data showed that protein level of phosphorylated AKT (p-AKT) was elevated in the OA pretreatment groups (Fig. 4A and B). Meanwhile, we noticed that the phosphorylation of eNOS (p-eNOS) was higher in the OA pretreatment groups than that in the model group (Fig. 4C and D).

Discussion

AS is an arteriosclerotic vascular disease in endothelial cells. Diabetes is one of the major risk factors for the formation of AS (41). Recently, OA has attracted much attention in protecting against AS (42,43).

In the presented study, we found that OA could improve cell viability of HUVECs that was declined by the high glucose treatment, suggesting a protective effect of OA on HUVECs. To explore the role of OA in high-glucose mediated injury of HUVECs, we detected the oxidative response of HUVECs after the treatment with OA. The results showed that OA recovered the NO generation and decreased MDA content. The activities of SOD and CAT were higher in the OA pretreatment groups than those in the model group, indicating that OA had a potential of protecting against the hyperglycemia injury in diabetes via suppressing the oxidative stress. The cell viability is largely dependent on the function of mitochondria (44). Thus, we detected the function of mitochondria by estimating the ROS production and MMP. Interestingly, our results revealed that ROS burst and MMP loss caused by high glucose were alleviated in the OA pretreatment groups. Moreover, apoptosis was reported to be closely related to oxidative stress (45). Therefore, the apoptosis of HUVECs was detected by flow cytometry assay. Results showed that apoptosis of HUVECs caused by high glucose was depressed by OA. Additionally, it is well known that caspase-3 (46), Fas and Fasl (47) act as pro-apoptotic signals. Bcl-2 (48) is considered as an important anti-apoptotic factor. We found that the expressions of caspase-3, Fas and Fasl decreased in the OA pretreatment groups both in the transcriptional and translated levels. Conversely, the expression of Bcl-2 increased in the OA pretreatment groups in comparison to the model group, indicating that OA depressed the cell apoptosis of HUVECs by modulating the expression of apoptosis-related factors.

Furthermore, according to previous study, AKT/eNOS contributes to the prevention of apoptosis in endothelial cells (49). Another previous study pointed out that the phosphorylation of AKT/eNOS was decreased by high glucose in HUVECs (50). To illustrate the action mechanism of OA underlying the high glucose-induced HUVECs injury, we examined the activity of AKT/eNOS signaling. The results showed that the pretreatment of OA increased the levels of phosphorylated AKT (p-AKT) and phosphorylated eNOS (p-eNOS) in comparison to model group. A previous study showed that the endothelial injury was alleviated through enhancing the activity of PI3K/Akt/eNOS signaling (51). Although the effects of OA in this study still needed further validation, it provided a new molecular insight for understanding the effects of OA on AS in diabetes. Furthermore, OA could exert anti-tumor effect by inhibiting the activation of Akt signaling (25,52). This was contrary to the activation of Akt signaling by OA in this study. These results seemed to be contradictory; however, they demonstrated the protective effect of OA. The distinct results may be attributed to different cell type and cell context. In addition, due to the complexity of signal transduction, the signal modulation net would be better understood with efforts from further studies.

In summary, OA alleviated the cell injury mediated by high glucose by improving the cell viability, increasing the NO content, decreasing MDA level and rescuing the activities of SOD and CAT. Moreover, the ROS burst and MMP loss caused by high glucose could be mitigated by OA. The apoptosis induced by high glucose was inhibited by OA via modulating the expressions of caspase-3, Fas, Fasl and Bcl-2. Furthermore, the protective effects of OA may be associated with the activation of AKT/eNOS signaling pathway. Collectively, our results provided inspiration of new therapeutic strategies for the treatment of AS on diabetics.