Journal of Diabetes Research

Journal of Diabetes Research / 2019 / Article
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Research Article | Open Access

Volume 2019 |Article ID 9696521 |

Jingjing Liu, Chunyu Jiang, Xu Ma, Lishuai Feng, Jianbo Wang, "Notoginsenoside Fc Accelerates Reendothelialization following Vascular Injury in Diabetic Rats by Promoting Endothelial Cell Autophagy", Journal of Diabetes Research, vol. 2019, Article ID 9696521, 16 pages, 2019.

Notoginsenoside Fc Accelerates Reendothelialization following Vascular Injury in Diabetic Rats by Promoting Endothelial Cell Autophagy

Guest Editor: Zhihong Peng
Received25 Mar 2019
Revised15 May 2019
Accepted29 Jul 2019
Published03 Sep 2019


Interventional therapies, such as percutaneous transluminal angioplasty and endovascular stent implantation, are used widely for the treatment of diabetic peripheral vascular complications. Reendothelialization is an essential process in vascular injury following interventional therapy, and hyperglycemia in diabetes mellitus (DM) plays an important role in damaging endothelial layer integrity, leading to the retardance of reendothelialization and excessive neointimal formation. Notoginsenoside Fc (Fc), a novel saponin isolated from Panax notoginseng, effectively counteracts platelet aggregation. Nevertheless, the potential effects and molecular mechanisms of Fc on reendothelialization have yet to be explored. In this study, we present novel findings that show the benefit of Fc in accelerating reendothelialization and alleviating excessive neointimal formation following carotid artery injury in diabetic Sprague–Dawley rats in vivo. Simultaneously, the decreased autophagy of the injured carotid artery in diabetic rats was restored by Fc treatment. Our in vitro results also demonstrated that Fc promoted endothelial cell proliferation and migration under high-glucose treatment by increasing autophagy. In summary, this study supported the notion that Fc could accelerate reendothelialization following vascular injury in diabetic rats by promoting autophagy, suggesting that Fc may exert therapeutic benefits for early endothelial injury and restenosis following intervention in diabetes-associated vascular diseases.

1. Introduction

Over 300,000,000 individuals have diabetes mellitus (DM) worldwide [1], and approximately 60–80% of DM patients present with vascular complications [2]. At present, interventional therapies, such as percutaneous transluminal angioplasty and endovascular stent implantation, have been widely used for the treatment of diabetic peripheral vascular complications and have shown promising results in clinical practice [3, 4]. However, vascular restenosis following intervention remains a serious problem in angioplasty treatment for diabetic peripheral artery diseases and the restenosis rate can reach as high as 50–70% [5].The main reason for this effect is that the drug-eluting stent or balloon not only inhibits the proliferation of smooth muscle cells but also inhibits reendothelialization, which is essential for the prevention of excessive neointima [6]. Therefore, new strategies for efficient reendothelialization are needed. Notoginsenoside Fc (Fc), a novel protopanaxadiol- (PPD-) type saponin isolated from the leaves of Panax notoginseng, effectively counteracts platelet aggregation [7]. There are multiple reports implicating other saponins derived from P. notoginseng in cardiovascular pathophysiology [8]. Dammarane-type triterpene saponins, including ginsenosides and notoginsenosides, contributed to the abovementioned pharmacological effects, and these saponins can be divided into PPD and protopanaxatriol (PPT) types based on their aglycone skeleton [9]. It has been demonstrated that Fc exhibits various pharmacological activities as a folk medicine or dietary supplement [10, 11]. However, little information regarding the effects of Fc on reendothelialization and the underlying mechanism is available.

Autophagy is an evolutionarily conserved catabolic process that mediates protein degradation, organelle turnover, and recycling of cytoplasmic contents in a lysosome-dependent manner [12]. Recent studies have shown that autophagic dysregulation is associated with several cardiovascular pathological processes, such as atherosclerosis, cardiac hypertrophy, and cardiomyopathies [13, 14]. Uberti et al. reported that vitamin D-activated autophagy promotes human umbilical vein endothelial cell survival under oxidative stress, suggesting that autophagy represents a target for endothelial cell protection [15]. Endothelial apoptosis interferes with endothelial regeneration and function, thus retarding the endothelial wound healing process [16]. Moreover, Ye et al. indicated that knockdown of Beclin 1, a key component in autophagy initiation, exacerbated neointimal formation after rat carotid injury, which was associated with retarded reendothelialization [17]. In addition, many studies have demonstrated that P. notoginseng protects many types of cells via autophagy induction [1820]. Therefore, in the present study, we investigated whether Fc protects against endothelial cell injury, accelerates reendothelialization, and attenuates excessive neointimal formation in DM rats via autophagy induction.

With this information, the present study is aimed at determining whether Fc accelerates reendothelialization and alleviates excessive neointimal formation following carotid artery injury in diabetic rats. We hypothesized that the underlying mechanism involves promoting autophagy in rat aortic endothelial cells (RAOECs).

2. Materials and Methods

2.1. Drug Preparation

Notoginsenoside Fc (chemical structure C58H98O26, molecular , and ) was purchased from Shanghai Yuanye Bio-Technology Co. Ltd. (Shanghai, China). The molecular structure is shown in Figure 1(a).

2.2. Animal Preparation

Animals and forage were purchased from the Model Animal Research Centre of Nanjing University (Jiangsu, China). This study conformed to the Guide for the Care and Use of Laboratory Animals published by the US National Institutes of Health (NIH publication no. 85-23, revised 1996), and the Institutional Animal Care and Use Committee of Shanghai Sixth People’s Hospital approved the protocol. All rats were housed in individually ventilated cages (three or four per cage) under specific pathogen-free conditions. Housing was temperature controlled, with a 12 h/12 h light/dark cycle. In total, 48 male Sprague–Dawley rats () were randomly separated into four groups: sham group (), control group (), DM group (), and DM+Fc group (). After 12 h of fasting, the DM and DM+Fc groups were given an intraperitoneal injection of 60 mg/kg streptozotocin (STZ). Fasting blood samples were taken from the tail vein of rats and the blood glucose levels of all rats were tested twice on the days 3 and 7, respectively, after STZ injection. A Roche blood glucose meter and Roche test paper were used to measure fasting blood glucose levels. A fasting blood , both on day 3 and day 7, represented successful establishment of a diabetic rat model.

2.3. Carotid Artery Injury and Evans Blue Staining

After successful modeling, animals were fasted without water deprivation for 12 h before wire injury of the rat carotid artery was performed as described previously [21]. A 2-French balloon catheter (Edwards Lifesciences, Irvine, CA, USA) was inserted through the left external carotid artery into the common carotid artery and insufflated three times with 2 atm of pressure. Following injury, the external carotid artery was rapidly ligated and blood flow was resumed. Then, the DM+Fc group began drug treatment with a gavage of 3.5 mg/kg/d Fc until the rats were killed. The other three groups were given the same dose of saline. A schematic diagram to illustrate the different experimental animal groups and treatments is showed in Figure 1(c). The reendothelialization rate was confirmed by Evans blue dye (Sigma-Aldrich, St. Louis, MO, USA) staining. The area of remaining denudation at 14 and 28 days after injury was determined by left thigh femoral vein injection of 0.5% Evans blue dye after the rat was anesthetized. Subsequently, the tissue was cut longitudinally, washed with phosphate-buffered saline (PBS), and fixed with 4% paraformaldehyde. Samples were photographed using a dissecting microscope. Deendothelialized areas were defined as areas that stained blue, as assessed using ImageJ software (NIH, Bethesda, MD, USA). Simultaneously, the blood glucose of the rats was measured at days 0 (before carotid artery injury), 14, and 28 (Figure 1(b)).

2.4. Hematoxylin and Eosin (HE) Staining

On day 28 after injury, rat arteries were harvested and embedded in paraffin for HE staining. Each specimen was incubated in 4% paraformaldehyde for 24–48 h and then embedded in paraffin. Paraffin sections (3–5 mm thick) were dewaxed, stained, examined microscopically, and photographed. Images were captured using a fluorescence microscope (Jenoptik, Jena, Germany) and analyzed using ImageJ software. Neointimal and media areas were computed as follows: .

2.5. Immunohistochemistry

At 14 days after injury, rat arteries were harvested and embedded in optimal cutting temperature (OCT) compound (Tissue-Tek; Sakura Finetek, Torrance, CA, USA), snap-frozen in liquid nitrogen, and stored at −80°C for further use. Then, 7 μm thick sections were cut at 500 mm intervals of the injured carotid artery (4 mm) and sections from the middle of the segments were stained with HE for immunohistochemistry. Samples were immunostained using a rabbit anti-Beclin 1 antibody (Cell Signaling Technology, Boston, MA, USA). The vessels were then stained with horse radish peroxidase-conjugated anti-rabbit IgG polymer and finally colored with 3,3-diaminobenzidin. Representative histological photomicrographs are shown.

2.6. Cell Culture

RAOECs were obtained from the American Type Culture Collection (Manassas, VA, USA). Cells were cultured in Dulbecco’s modified Eagle’s medium (DMEM) supplemented with 10% fetal bovine serum (Gibco, Carlsbad, CA, USA). RAOECs were cultivated in a humidified atmosphere at 37°C with 5% CO2. The growth medium was replaced every 2 days, and passages 4–6 were used for experiments. According to our previous experiments [22], the cells were divided into the following groups: (i) normal glucose (NG) group: cells were incubated in DMEM containing 5.6 mM D-glucose; (ii) NG+Fc group: cells were treated with DMEM and 20 μM Fc for 24 h; (iii) high-glucose (HG) group: cells were treated with 30 mM D-glucose for 24 h; and (iv) HG+Fc group: cells were treated with 30 mM D-glucose and 20 μM Fc for 24 h. In addition, cells were pretreated with 5 mM 3-methyladenine (3-MA) (Selleck Chemicals, Houston, TX, USA) for 2 h to inhibit autophagy.

2.7. Cell Proliferation Assay

RAOECs were seeded onto a 96-well plate with cells per well. After growing to 70–80% confluence, cells were treated with the corresponding drugs for 24 h. Cell cycle analyses were performed using the Cell Cycle Phase Determination Kit (Yeasen) according to the manufacturer’s instructions. Each experiment was performed independently at least three times.

2.8. Wound Healing Assay

The cell wound healing assay was employed to measure cell migration. RAOECs were inoculated into 6-well plates ( cells/well) and grown for 24 h to reach 70–80% confluence. Following 12 h of serum withdrawal, three scratches were made in each well using a P-20 pipette. Cells were incubated for 24 h with the indicated treatment to enable migration, and images of each well were taken to measure gap changes in the scratches.

2.9. Monitoring Autophagy Flux Using the mRFP-eGFP-LC3B Plasmid

RAOECs were individually seeded onto 35 mm glass bottom dishes for confocal microscopy. When cells grew to 80% confluence, the original medium was discarded; 4 μg of the mRFP-eGFP-LC3B plasmid (GenePharma, Shanghai, China) was dissolved in the Opti-MEM reduced serum medium and then mixed with 5 μL of liposomes using Lipofectamine® 2000 Reagent (Invitrogen, Carlsbad, CA, USA). The mixture was added to the cells and replaced with serum medium after 4–6 h. Finally, cells were immobilized by 4% paraformaldehyde for 20 min and washed three times with PBS after 48 h. For nuclear staining, cells were stained with DAPI for 15 min in the dark. Samples were observed and photographed with a confocal microscope (LSM 710 META; Zeiss, Oberkochen, Germany). At least eight cells (per experiment) were randomly selected to determine the number of mRFP-LC3B or eGFR-LC3B puncta in each group, and the numbers of red and yellow puncta were counted as previously described [23].

2.10. Transmission Electron Microscopy

RAOECs were immobilized by glutaraldehyde in an atmosphere of 4°C. After ethanol dehydration and embedding in epoxy resin, ultrathin sections were prepared using an LKB2-III ultrathin microtome and stained with both uranyl acetate and lead citrate. Changes in the cellular ultrastructure were observed and photographed with an EM420 transmission electron microscope.

2.11. Reverse Transcription-Quantitative PCR (RT-qPCR)

Total RNA was extracted with TRIzol reagent (Invitrogen) from RAOECs. The concentration of the isolated RNA sample was measured using a NanoDrop 2000 (Thermo Fisher Scientific, Carlsbad, CA, USA) and then reverse transcribed to obtain complementary DNA using a PrimeScript RT Reagent Kit (TaKaRa, Dalian, China). PCR was then performed using SYBR Premix Ex Taq (TaKaRa) with LC3B-, Beclin 1-, p62-, and GAPDH-specific primers. The primer pairs were as follows: LC3B: 5-TACGAGAGCGAGAGAGATGAA-3 (forward) and 5-GCCTTCAGAGCTGACATGTAT-3 (reverse); Beclin 1: 5-ATGCCCACTTCAGCATCTC-3 (forward) and 5-TCACTGTCTTCCTCCTCTACTT-3 (reverse); p62: 5-CTGATCCCTGTCAAGCAGTATC-3 (forward) and 5-AGATCTTTGCACCAGTCTCTTC-3 (reverse); GAPDH (internal control): 5-GCAAGGATACTGAGAGCAAGAG-3 (forward) and 5-GGATGGAATTGTGAGGGAGATG-3 (reverse). Relative mRNA expression levels were normalized to GAPDH and are presented as values.

2.12. Western Blot Analysis

The carotid arteries of rats or cells were lysed with cell lysis buffer (Beyotime Institute of Biotechnology) supplemented with 0.5 mM phenylmethanesulfonylfluoride. Following centrifugation (12,000 rpm, 15 min, 4°C), protein concentrations were determined using a Bicinchoninic Acid Protein Assay Kit (Beyotime Institute of Biotechnology). The same mass of total protein was separated by sodium dodecyl sulfate-polyacrylamide gel electrophoresis and transferred to polyvinylidene difluoride membranes (0.22; Millipore, Billerica, MA, USA). Membranes were blocked with 5% nonfat milk in Tris-buffered saline containing 0.1% Tween 20 for 2 h at room temperature. Membrane-bound proteins were probed with the indicated primary antibody (1 : 500–1 : 1,000 dilution) overnight at 4°C, followed by horseradish peroxidase-conjugated secondary antibodies (1 : 5,000; Proteintech, Chicago, IL, USA) at room temperature for 1 h. Protein bands were detected with an enhanced chemiluminescence detection kit (Cell Signaling Technology) and photographed using a GE Amersham Imager 600 imaging system (GE Life Sciences, Chicago, IL, USA). Antibodies against LC3B (cat. no. 2775S), p62 (cat. no. 5114S), Beclin 1 (cat. no. 3738S), PCNA (cat. no. 13110S), and β-actin (cat. no. 4970S) were purchased from Cell Signaling Technology.

2.13. Statistical Analysis

All data were from at least three independent experiments and are presented as the deviation. Statistical analyses involving multiple groups were performed by one-way analysis of variance followed by the least significant difference test using SPSS software (ver. 20.0; IBM Corp., Armonk, NY, USA). was considered statistically significant.

3. Results

3.1. Fc Accelerates Reendothelialization following Carotid Artery Injury in Diabetic Sprague–Dawley Rats

To explore the effects of Fc on endothelial repair ability following vascular wire injury in vivo, we used Evans blue staining to examine reendothelialization of the carotid arteries in rats. As shown in Figure 2, the endothelium was gradually regenerated after injury and the reendothelialization rate reached by day 14 and by day 28, identical to noninjured sham rats. In diabetic rats, the reendothelialization rate was only by day 14 and by day 28, which was significantly retarded compared to the injured control. However, the repair capability of the injured artery was markedly improved by treatment with Fc. In the DM+Fc group, the reendothelialization rate was by day 14 and by day 28.

3.2. Fc Retards Excessive Neointimal Formation following Carotid Artery Injury in Diabetic Sprague–Dawley Rats

Neointima formation in wire-injured carotid arteries of rats was determined using cross sections of carotid arteries by HE staining at 14 days after vascular wire injury and Fc treatment. The neointima area, media area, and neointima-to-media area ratios were analyzed. As shown in Figure 3(a), diabetes significantly increased neointimal hyperplasia compared to the control group. The neointima area (Figure 3(b)) and neointima-to-media area ratios (Figure 3(d)) of injured carotid arteries were significantly increased in rats of the DM group compared to the control group. In contrast, the severe neointimal hyperplasia was attenuated by Fc treatment and the neointima area and neointima-to-media area ratios were decreased in rats of the DM+Fc group compared to the DM group. The media area did not differ significantly among the four groups (Figure 3(c)). Moreover, we found that the neointimal hyperplasia area was inversely associated with the reendothelialization rate.

3.3. Fc Increases Beclin 1 Protein of the Intima following Carotid Artery Injury in Diabetic Sprague–Dawley Rats

The effects of Fc on Beclin 1 protein of the intima following carotid artery injury were detected by immunohistochemistry. As shown in Figure 4(a), Beclin 1 protein was found predominantly in the intima. The number of Beclin 1-positive cells was decreased in the DM group rats compared to the control group rats; however, the expression of Beclin 1 of the injured artery was markedly improved by treatment with Fc (Figure 4(b)).

3.4. Fc Prevents HG-Induced Autophagy Reduction in Endothelial Cells

The effects of Fc on autophagy in RAOECs were first examined by measuring the following autophagy-related markers via Western blot and RT-qPCR analysis: LC3B, Beclin 1, and p62. As shown in Figure 5, HG decreased both protein and mRNA expression of LC3B and Beclin 1 and increased the level of p62. Fc treatment markedly upregulated the expression of LC3B and Beclin 1 and downregulated that of p62 in RAOECs compared to the HG group. To further confirm Fc-induced autophagy in RAOECs, the mRFP-eGFP-LC3B plasmid was transfected into cells and visualized by confocal microscopy. Yellow puncta, reflective of the combination of red fluorescent protein (RFP) and green fluorescent protein (GFP) fluorescence, indicate autophagosomes, which are membrane-bound structures that sequester cellular components, whereas red puncta (RFP only) indicate autolysosomes [24]. Both red and yellow puncta decreased significantly in the HG-treated group compared with the NG group; however, pretreatment with Fc followed by HG increased yellow puncta with no obvious difference in red puncta (Figures 6(a) and 6(b)). Transmission electron microscopy was used to observe autophagosomes when autophagy occurred. Small vacuoles were present in HG-treated RAOECs, but the number increased when the cells were pretreated with Fc (Figures 6(c) and 6(d)).

3.5. Fc Promotes RAOEC Proliferation and Migration under HG Conditions via Autophagy

The effects of Fc-induced autophagy in RAOECs were further confirmed by evaluating Fc-induced cell proliferation and migration after autophagy inhibition. RAOEC proliferation was detected by cell cycle progression analysis (Figures 7(a) and 7(b)). In addition, the protein expression of proliferating cell nuclear antigen (PCNA) was detected by Western blot analysis (Figure 7(e)). More RAOECs were arrested in the G1 phase, and the protein expression of PCNA was lower in HG-treated cells than in NG cells. Fc promoted the proliferation of RAOECs by reversing these changes but decreased following pretreatment with the autophagy inhibitor, 3-MA (5 mM, 2 h). Cell migration was examined using the cell wound healing assay (Figures 7(c) and 7(d)). The migration of RAOECs under HG conditions was significantly reduced compared to NG; cell migration was increased in the HG+Fc group compared to the HG group. However, migration decreased following the addition of 3-MA. Furthermore, cell proliferation and migration did not differ significantly among the NG, NG+Fc, and NG+Fc+3-MA groups.

4. Discussion

Hyperglycemia is thought to play an important role in DM by increasing the expression of mitogenic growth factors and inflammatory mediators; during this process, diabetic vascular complications may occur, such as atherosclerosis, diabetic nephropathy, diabetic retinopathy, or myocardial infarction [25]. Interventional surgery has become an important treatment for diabetic vascular complications. Inevitably, it results in vascular endothelium injury, leading to vascular endothelial cell dysfunction [26]. A number of studies have shown that it is of great significance in the prevention of interventional restenosis to form a functional and intact endothelial monolayer early at the injury site, namely, reendothelialization [2729]. In addition, hyperglycemia in DM plays an essential role in damaging endothelial layer integrity, leading to endothelial dysfunction and injury [25].

Notoginsenoside Fc is the unique ingredient of P. notoginseng that is commonly used as a platelet aggregation inhibitor or as a blood coagulation inhibitor to prevent or treat thrombotic diseases [10]. Fc has been demonstrated to have a slow elimination from plasma, with a long half-life (22–30 h). When given orally, Fc showed dose-independent pharmacokinetic characteristics and its oral bioavailability was 0.10–0.14% [10]. In addition, Ju et al. indicated that notoginsenoside Fc showed relatively higher exposure in rat plasma after oral administration of saponins from P. notoginseng leaves compared with other saponins [7]. Previous studies have reported that improved reendothelialization without platelet adhesion is essential to enhance the long-term patency of blood-contacting devices [30]. Tu et al. found that inhibiting platelet adhesion eventually accelerated the reendothelialization of titanium vascular implants [31]. Another study showed that a bioactive stent surface coating promoted endothelialization while preventing platelet adhesion [32]. Therefore, it is reasonable that Fc compromised endothelial cell repair and accelerated reendothelialization in diabetic rats both in vitro and in vivo. To our knowledge, this is the first study to demonstrate that Fc accelerates reendothelialization, suggesting that Fc could be developed as a novel therapeutic agent for the prevention and treatment of postinjury restenosis in diabetic vascular complications. The present study focused on reendothelialization, or the repair of endothelial cells after interventional injury. In contrast, in our previous study, which focused on the preventive effect of Fc on endothelial cell injury under HG, Fc alleviated atherosclerosis in diabetic rats [22].

In our in vivo experiment, diabetes was established by injection of high doses of STZ. Wire injury of the rat carotid artery was used to simulate vascular injury after intervention. Endothelial recovery, or reendothelialization, after vascular injury (i.e., balloon angioplasty or stent implantation) is clinically relevant to promote vascular healing and to prevent excessive neointimal formation [33]. Meanwhile, studies using animal models have also indicated that delayed endothelial recovery correlates with increased neointimal hyperplasia after vascular injury [34, 35]. Evans blue staining is a reliable way to detect reendothelialization [36]. Our results confirmed that Fc treatment following rat carotid artery injury accelerated endothelial repair and alleviated neointimal hyperplasia in DM rats. These data support the beneficial effects of the use of Fc to prevent postinjury restenosis in diabetes.

Next, we investigated how Fc affected reendothelialization and ultimately neointimal formation. Autophagy plays a crucial role in maintaining endothelial integrity and promoting endothelial repair [17]. Du et al. reported that autophagy may be an important promoter of angiogenesis, as both pharmacological inhibition and genetic inhibition of autophagy significantly impair migration in endothelial cells [37]. In addition, we found that Fc attenuated HG-induced vascular endothelial cell injury via upregulation of PPAR-γ in diabetic rats. Furthermore, PPAR-γ mediated autophagy and Yuan et al. indicated that PPAR-γ signaling inhibited cardiac hypertrophy via activation of autophagy [38]. Beclin 1 levels were detected in vivo by immunohistochemistry. Beclin 1 is a mammalian autophagy gene that is central to autophagy regulation [17]. It was found predominantly in the intima of the vasculature. The results indicated that autophagy of injured carotid arteries was decreased in the DM group compared to the control group; however, autophagy was markedly improved following Fc treatment. Three different approaches were used in vitro to determine the role of autophagy in RAOECs. During autophagy, the cytosolic form of LC3B-I is converted into LC3B-II, a phosphatidylethanolamine-conjugated form, to promote autophagosome formation, and the amount of LC3B-II is a commonly used indicator of autophagy [39]. In this study, protein and mRNA levels of LC3B-II and Beclin 1 were determined by Western blot and RT-qPCR analysis. Both were decreased under HG conditions but increased following treatment with Fc. In addition, p62, an autophagic substrate, whose level inversely correlates with autophagic flux [40], was downregulated after Fc treatment. When cells are transfected with LC3B constructed with the GFP and RFP plasmid (mRFP-eGFP-LC3B), autophagosome formation and autophagy flux can be visualized via yellow and red puncta [41]. Our data suggested a decrease in the number of autophagosomes and autolysosomes in the HG group but an increase in autophagosomes only in the HG+Fc group. Autophagy was simultaneously observed by transmission electron microscopy, further confirming the increased number of autophagosomes induced by Fc under HG conditions. Together, these findings support Fc-dependent prevention of HG-induced autophagy reduction in endothelial cells and that the target may be prior to the formation of autophagosomes.

The disruption of endothelial monolayer integrity induced by hyperglycemia in DM can be alleviated by the proliferation and migration of neighboring endothelial cells [42]. We confirmed that Fc could promote RAOEC proliferation and migration under HG conditions. To future explore the link between Fc-induced autophagy and proliferation, we used a low concentration of 3-MA, a synthetic intermediate, and cell-permeable autophagic sequestration blocker. We found that Fc-induced proliferation and migration were reversed when autophagy was inhibited, suggesting that Fc promotes RAOEC proliferation and migration under HG conditions via autophagy.

There were limitations to this study. First, we used only one dose of Fc in the in vivo study. Therefore, the dose-dependent effects of Fc in vivo should be examined in a future study. Second, the blood concentration and bioavailability of Fc were not measured in the animals and these should also be examined. Therefore, the applicability of Fc to early endothelial injury and restenosis following intervention in diabetic vascular complications needs to be further investigated.

5. Conclusions

In conclusion, notoginsenoside Fc is a relatively new and slightly studied saponin isolated from P. notoginseng. Our study is the first to report that Fc can promote endothelial cell proliferation and migration under HG conditions in vitro, ultimately accelerating reendothelialization in the peripheral vascular system of diabetic rats in vivo by promoting autophagy. These data suggest that Fc exerts a potential therapeutic benefit for early endothelial injury and restenosis following intervention in diabetes-associated peripheral vascular diseases.

Data Availability

All data used to support the findings of this study are included within the article.

Conflicts of Interest

The authors declare no conflict of interest.


This study was supported by grants from the Shanghai Science and Technology Committee Research Project (Grant no. 17411966700).


  1. J. Gong, K. Fang, H. Dong, D. Wang, M. Hu, and F. Lu, “Effect of fenugreek on hyperglycaemia and hyperlipidemia in diabetes and prediabetes: a meta-analysis,” Journal of Ethnopharmacology, vol. 194, pp. 260–268, 2016. View at: Publisher Site | Google Scholar
  2. C. M. Lee, R. R. Huxley, T. H. Lam et al., “Prevalence of diabetes mellitus and population attributable fractions for coronary heart disease and stroke mortality in the WHO South-East Asia and Western Pacific regions,” Asia Pacific Journal of Clinical Nutrition, vol. 16, no. 1, pp. 187–192, 2007. View at: Google Scholar
  3. Y. Q. Zhu, J. G. Zhao, F. Liu et al., “Subintimal angioplasty for below-the-ankle arterial occlusions in diabetic patients with chronic critical limb ischemia,” Journal of Endovascular Therapy, vol. 16, no. 5, pp. 604–612, 2009. View at: Publisher Site | Google Scholar
  4. J. Wang, Y. Q. Zhu, J. G. Zhao et al., “Infrapopliteal angioplasty with a long over-the-wire (OTW) balloon in the treatment of severe limb ischemia in diabetic patients: a retrospective study,” Acta Radiologica, vol. 50, no. 4, pp. 360–367, 2009. View at: Publisher Site | Google Scholar
  5. M. Fujihara, M. Takahara, S. Sasaki et al., “Angiographic dissection patterns and patency outcomes after balloon angioplasty for superficial femoral artery disease,” Journal of Endovascular Therapy, vol. 24, no. 3, pp. 367–375, 2017. View at: Publisher Site | Google Scholar
  6. A. V. Finn, M. Joner, G. Nakazawa et al., “Pathological correlates of late drug-eluting stent thrombosis: strut coverage as a marker of endothelialization,” Circulation, vol. 115, no. 18, pp. 2435–2441, 2007. View at: Publisher Site | Google Scholar
  7. Z. Ju, J. Li, H. Han, L. Yang, and Z. Wang, “Analysis of bioactive components and multi-component pharmacokinetics of saponins from the leaves of Panax notoginseng in rat plasma after oral administration by LC-MS/MS,” Journal of Separation Science, vol. 41, no. 7, pp. 1512–1523, 2018. View at: Publisher Site | Google Scholar
  8. B. Sun, J. Xiao, X. B. Sun, and Y. Wu, “Notoginsenoside R1 attenuates cardiac dysfunction in endotoxemic mice: an insight into oestrogen receptor activation and PI3K/Akt signalling,” British Journal of Pharmacology, vol. 168, no. 7, pp. 1758–1770, 2013. View at: Publisher Site | Google Scholar
  9. L. W. Qi, C. Z. Wang, and C. S. Yuan, “Isolation and analysis of ginseng: advances and challenges,” Natural Product Reports, vol. 28, no. 3, pp. 467–495, 2011. View at: Publisher Site | Google Scholar
  10. C. He, J. Li, N. Xu et al., “Pharmacokinetics, bioavailability, and metabolism of notoginsenoside Fc in rats by liquid chromatography/electrospray ionization tandem mass spectrometry,” Journal of Pharmaceutical and Biomedical Analysis, vol. 109, pp. 150–157, 2015. View at: Publisher Site | Google Scholar
  11. L. J. Ma, F. Liu, Z. F. Zhong, and J. B. Wan, “Comparative study on chemical components and anti-inflammatory effects of Panax notoginseng flower extracted by water and methanol,” Journal of Separation Science, vol. 40, no. 24, pp. 4730–4739, 2017. View at: Publisher Site | Google Scholar
  12. D. J. Klionsky and S. D. Emr, “Autophagy as a regulated pathway of cellular degradation,” Science, vol. 290, no. 5497, pp. 1717–1721, 2000. View at: Publisher Site | Google Scholar
  13. A. M. Choi, S. W. Ryter, and B. Levine, “Autophagy in human health and disease,” The New England Journal of Medicine, vol. 368, no. 19, pp. 1845-1846, 2013. View at: Publisher Site | Google Scholar
  14. S. Lavandero, M. Chiong, B. A. Rothermel, and J. A. Hill, “Autophagy in cardiovascular biology,” The Journal of Clinical Investigation, vol. 125, no. 1, pp. 55–64, 2015. View at: Publisher Site | Google Scholar
  15. F. Uberti, D. Lattuada, V. Morsanuto et al., “Vitamin D protects human endothelial cells from oxidative stress through the autophagic and survival pathways,” The Journal of Clinical Endocrinology & Metabolism, vol. 99, no. 4, pp. 1367–1374, 2014. View at: Publisher Site | Google Scholar
  16. X. Y. Zhang, C. Su, Z. Cao et al., “CXCR7 upregulation is required for early endothelial progenitor cell–mediated endothelial repair in patients with hypertension,” Hypertension, vol. 63, no. 2, pp. 383–389, 2014. View at: Publisher Site | Google Scholar
  17. L. X. Ye, J. Yu, Y. X. Liang, J. S. Zeng, R. X. Huang, and S. J. Liao, “Beclin 1 knockdown retards re-endothelialization and exacerbates neointimal formation via a crosstalk between autophagy and apoptosis,” Atherosclerosis, vol. 237, no. 1, pp. 146–154, 2014. View at: Publisher Site | Google Scholar
  18. L. Qiao, X. Zhang, M. Liu et al., “Ginsenoside Rb1 enhances atherosclerotic plaque stability by improving autophagy and lipid metabolism in macrophage foam cells,” Frontiers in Pharmacology, vol. 8, p. 727, 2017. View at: Publisher Site | Google Scholar
  19. G. Huang, B. Zou, J. Lv et al., “Notoginsenoside R1 attenuates glucose-induced podocyte injury via the inhibition of apoptosis and the activation of autophagy through the PI3K/Akt/mTOR signaling pathway,” International Journal of Molecular Medicine, vol. 39, no. 3, pp. 559–568, 2017. View at: Publisher Site | Google Scholar
  20. W. Xing, L. Yang, Y. Peng et al., “Ginsenoside Rg3 attenuates sepsis-induced injury and mitochondrial dysfunction in liver via AMPK-mediated autophagy flux,” Bioscience Reports, vol. 37, no. 4, 2017. View at: Publisher Site | Google Scholar
  21. T. Kessler, L. Zhang, Z. Liu et al., “ADAMTS-7 inhibits re-endothelialization of injured arteries and promotes vascular remodeling through cleavage of thrombospondin-1,” Circulation, vol. 131, no. 13, pp. 1191–1201, 2015. View at: Publisher Site | Google Scholar
  22. J. Liu, C. Jiang, X. Ma, and J. Wang, “Notoginsenoside Fc attenuates high glucose-induced vascular endothelial cell injury via upregulation of PPAR-γ in diabetic Sprague–Dawley rats,” Vascular Pharmacology, vol. 109, pp. 27–35, 2018. View at: Publisher Site | Google Scholar
  23. J.-H. Lu, J.-Q. Tan, S. S. K. Durairajan et al., “Isorhynchophylline, a natural alkaloid, promotes the degradation of alpha-synuclein in neuronal cells via inducing autophagy,” Autophagy, vol. 8, no. 1, pp. 98–108, 2012. View at: Publisher Site | Google Scholar
  24. Y. Ikeda, A. Shirakabe, Y. Maejima et al., “Endogenous Drp1 mediates mitochondrial autophagy and protects the heart against energy stress,” Circulation Research, vol. 116, no. 2, pp. 264–278, 2015. View at: Publisher Site | Google Scholar
  25. K. A. Krychtiuk, S. P. Kastl, W. S. Speidl, and J. Wojta, “Inflammation and coagulation in atherosclerosis,” Hämostaseologie, vol. 33, no. 04, pp. 269–282, 2013. View at: Publisher Site | Google Scholar
  26. S. Zhang, N. Cui, Y. Wu, W. Zhong, C. M. Johnson, and C. Jiang, “Optogenetic intervention to the vascular endothelium,” Vascular Pharmacology, vol. 74, pp. 122–129, 2015. View at: Publisher Site | Google Scholar
  27. M. M. Thompson, J. S. Budd, S. L. Eady et al., “Platelet deposition after angioplasty is abolished by restoration of the endothelial cell monolayer,” Journal of Vascular Surgery, vol. 19, no. 3, pp. 478–486, 1994. View at: Publisher Site | Google Scholar
  28. D. He, M. Zhao, C. Wu et al., “Apolipoprotein A-1 mimetic peptide 4F promotes endothelial repairing and compromises reendothelialization impaired by oxidized HDL through SR-B1,” Redox Biology, vol. 15, pp. 228–242, 2018. View at: Publisher Site | Google Scholar
  29. W. Sun, Y. Huang, T. Yin et al., “Effects of elemene on inhibiting proliferation of vascular smooth muscle cells and promoting reendothelialization at the stent implantation site,” Biomaterials Science, vol. 5, no. 6, pp. 1144–1155, 2017. View at: Publisher Site | Google Scholar
  30. H. W. Jun and J. L. West, “Modification of polyurethaneurea with PEG and YIGSR peptide to enhance endothelialization without platelet adhesion,” Journal of Biomedical Materials Research. Part B, Applied Biomaterials, vol. 72B, no. 1, pp. 131–139, 2005. View at: Publisher Site | Google Scholar
  31. Q. Tu, Y. Zhao, X. Xue, J. Wang, and N. Huang, “Improved endothelialization of titanium vascular implants by extracellular matrix secreted from endothelial cells,” Tissue Engineering Part A, vol. 16, no. 12, pp. 3635–3645, 2010. View at: Publisher Site | Google Scholar
  32. S. R. Meyers, D. J. Kenan, X. Khoo, and M. W. Grinstaff, “Bioactive stent surface coating that promotes endothelialization while preventing platelet adhesion,” Biomacromolecules, vol. 12, no. 3, pp. 533–539, 2011. View at: Publisher Site | Google Scholar
  33. K. Grote, K. Sonnenschein, P. R. Kapopara et al., “Toll-like receptor 2/6 agonist macrophage-activating lipopeptide-2 promotes reendothelialization and inhibits neointima formation after vascular injury,” Arteriosclerosis, Thrombosis, and Vascular Biology, vol. 33, no. 9, pp. 2097–2104, 2013. View at: Publisher Site | Google Scholar
  34. H. Wang, X. Jiang, F. Yang et al., “Cyclin A transcriptional suppression is the major mechanism mediating homocysteine-induced endothelial cell growth inhibition,” Blood, vol. 99, no. 3, pp. 939–945, 2002. View at: Google Scholar
  35. R. Hutter, F. E. Carrick, C. Valdiviezo et al., “Vascular endothelial growth factor regulates reendothelialization and neointima formation in a mouse model of arterial injury,” Circulation, vol. 110, no. 16, pp. 2430–2435, 2004. View at: Publisher Site | Google Scholar
  36. X. Ke, X. R. Shu, F. Wu et al., “Overexpression of the β2AR gene improves function and re-endothelialization capacity of EPCs after arterial injury in nude mice,” Stem Cell Research & Therapy, vol. 7, no. 1, p. 73, 2016. View at: Publisher Site | Google Scholar
  37. J. Du, R.-J. Teng, T. Guan et al., “Role of autophagy in angiogenesis in aortic endothelial cells,” American Journal of Physiology-Cell Physiology, vol. 302, no. 2, pp. C383–C391, 2012. View at: Publisher Site | Google Scholar
  38. S. Yuan, J. Jin, L. Chen, Y. Hou, and H. Wang, “Naoxintong/PPARγ signaling inhibits cardiac hypertrophy via activation of autophagy,” Evidence-Based Complementary and Alternative Medicine, vol. 2017, Article ID 3801976, 9 pages, 2017. View at: Publisher Site | Google Scholar
  39. Y. Kabeya, N. Mizushima, T. Ueno et al., “LC3, a mammalian homologue of yeast Apg8p, is localized in autophagosome membranes after processing,” The EMBO Journal, vol. 19, no. 21, pp. 5720–5728, 2000. View at: Publisher Site | Google Scholar
  40. N. Mizushima, T. Yoshimori, and B. Levine, “Methods in mammalian autophagy research,” Cell, vol. 140, no. 3, pp. 313–326, 2010. View at: Publisher Site | Google Scholar
  41. Y. Kouroku, E. Fujita, I. Tanida et al., “ER stress (PERK/eIF2α phosphorylation) mediates the polyglutamine-induced LC3 conversion, an essential step for autophagy formation,” Cell Death & Differentiation, vol. 14, no. 2, pp. 230–239, 2007. View at: Publisher Site | Google Scholar
  42. J. Kang, H. L. Kim, J. B. Seo, J. Y. Lee, M. K. Moon, and W. Y. Chung, “Endothelial function estimated by digital reactive hyperemia in patients with atherosclerotic risk factors or coronary artery disease,” Heart and Vessels, vol. 33, no. 7, pp. 706–712, 2018. View at: Publisher Site | Google Scholar

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