Oxidative Medicine and Cellular Longevity

Oxidative Medicine and Cellular Longevity / 2020 / Article

Research Article | Open Access

Volume 2020 |Article ID 2468031 | 17 pages | https://doi.org/10.1155/2020/2468031

Wenxin Keli Regulates Mitochondrial Oxidative Stress and Homeostasis and Improves Atrial Remodeling in Diabetic Rats

Academic Editor: Laura Bravo
Received16 Oct 2019
Revised07 Jan 2020
Accepted25 Jan 2020
Published13 Feb 2020


Mitochondrial dysfunction and oxidative stress play an important role in the pathogenesis of both atrial fibrillation (AF) and diabetes mellitus (DM). Wenxin Keli (WXKL), an antiarrhythmic traditional Chinese medicine, has been shown to prevent cardiac arrhythmias through modulation of cardiac ion channels. This study tested the hypothesis that WXKL can improve atrial remodeling in diabetic rats by restoring mitochondrial function. Primary atrial fibroblasts of neonatal SD rats were divided into four groups: control, hydrogen peroxide (H2O2), H2O2+WXKL 1 g/L, and H2O2+WXKL 3 g/L groups. Intracellular mitochondrial membrane potential (MMP), reactive oxygen species (ROS), and mitochondrial oxygen consumption were measured. SD male rats were randomly divided into three groups: control, DM, and DM+WXKL groups. Rats in the DM+WXKL group were treated with daily gavage of WXKL at 3 g/kg. After eight weeks, echocardiography, hemodynamic examination, histology, electrophysiology study, mitochondrial respiratory function, and western blots were assessed. H2O2 treatment led to increased ROS and decreased intracellular MMP and mitochondrial oxygen consumption in primary atrial fibroblasts. WXKL improved the above changes. DM rats showed increased atrial fibrosis, greater left atrial diameter, lower atrial conduction velocity, higher conduction heterogeneity, higher AF inducibility, and lower mitochondrial protein expression, and all these abnormal changes except for left atrial diameter were improved in the DM+WXKL group. WXKL improves atrial remodeling by regulating mitochondrial function and homeostasis and reducing mitochondrial ROS in diabetic rats.

1. Introduction

Atrial fibrillation (AF) is the most common arrhythmia observed in the clinic. In recent years, its prevalence has increased with the aging of the population. AF is a risk factor for thromboembolism, which increases the risk of stroke and all-cause mortality [1, 2]. The development of AF is characterized by structural, electrical, and metabolic remodeling of the atria [3]. Previous studies have demonstrated that the development of AF is related to a variety of risk factors, but the pathogenesis of AF is complex and remains incompletely understood.

Diabetes mellitus (DM) is an independent risk factor for AF [4, 5]. Our previous work and those of other groups have demonstrated the importance of mitochondrial dysfunction and oxidative stress in mediating atrial remodeling in DM, which is associated with higher AF incidence [6]. Mitochondrial dysfunction is associated with the excessive release of reactive oxygen species (ROS) and cytochrome c, which initiates apoptosis. Abnormal biomarkers of oxidative stress have been found in AF patients and animal models of AF [7]. For example, the oxidative ratio of serum glutathione and cysteine in AF patients was significantly elevated. Prooxidative genes were upregulated, and antioxidant genes were downregulated in atrial appendages of AF patients [8, 9]. Montaigne et al. showed that mitochondrial dysfunction of atrial muscle before cardiac surgery was associated with the development of postoperative AF [10]. Currently, antioxidant drugs have been a potential therapeutic strategy of AF. Mitochondria play a vital role in myocardial energy metabolism and redox equilibrium. Energy metabolism disorder affects myocardial excitability and contraction. Therefore, cardiac mitochondria may be a specific therapeutic target.

Wenxin Keli (WXKL) is a traditional Chinese medicine, which is composed of Codonopsis, Rhizoma Polygonati, Notoginseng, Amber, and Nardostachys [11]. In Chinese medicine clinics, WXKL is used for the treatment of different cardiac arrhythmias, including AF. The antiarrhythmic effects of WXKL have been attributed to shortening of the action potential duration with simultaneous prolongation of the atrial effective refractory period. This leads to postrepolarization refractoriness, which can effectively prevent AF. WXKL exerts atrial-selective inhibition of peak Na current () and thus effectively suppresses AF in experimental models of AF [1214]. Our previous clinical study demonstrated that WXKL combined with amiodarone markedly shortened conversion time with no adverse reactions or proarrhythmic effects for AF patients [15]. WXKL was also used with other antiarrhythmic drugs in the clinic to prevent the perpetuation of AF [16].

Hydrogen peroxide (H2O2) as a potent oxidant induces mitochondrial dysfunction by increasing ROS production, which leads to reduced antioxidant activity and induced mitochondrial apoptotic signaling [17, 18]. High-fat diet- (HFD-) and low-dose streptozotocin- (STZ-) treated rats provide an animal model for type 2 DM (T2DM) [19]. The HFD+STZ model, which progresses from insulin resistance to hypoinsulinemia and hyperglycaemia, mimics the natural T2DM pathogenesis in humans and is suitable to investigate the pathogenesis of diabetic complications [19]. In this study, we aim to investigate the H2O2-induced oxidative stress in vitro and the atrial remodeling, atrial muscle mitochondrial function, and atrial electrophysiological properties in HFD/STZ-induced type 2 diabetic rats and the potential therapeutic effects of WXKL.

2. Materials and Methods

2.1. Isolation and Culturing of Fibroblasts

Primary cultures of atrial fibroblasts were isolated from 3-day-old neonatal Sprague-Dawley (SD) rats. In brief, neonatal SD rats were sacrificed by cervical dislocation, then sterilized in 75% ethanol, and subjected to subsequent operations in a clean bench. The left atrium was separated from the exposed heart; then, it was cut to small pieces of 1 mm3 and put in phosphate-buffered saline (PBS) solution without Ca2+ and Mg2+. Atrial tissues were repeat digested by trypsin type II collagenase buffer (0.125%, respectively) until the tissue completely dissipated. All the cell suspensions were centrifuged for 5 min at 1000 r/min. Isolated cells were resuspended in Dulbecco’s modified Eagle’s medium (DMEM), supplemented with 10% fetal bovine serum (FBS, Gibco) and 100 IU/mL penicillin-streptomycin (Gibco), and plated on 10 cm culture dishes for 2 h until the fibroblasts adhered to the dishes in a humidified atmosphere at 37°C under 5% CO2. The preseeding medium containing cardiomyocytes was removed, and the culture medium was added to continue to culture the atrial fibroblasts. The culture medium was changed every 48 hours. Atrial fibroblasts were used in subsequent experiments and incubated in FBS free medium for 24 h before treatment. The cells were pretreated with vehicle or WXKL (1 g/L or 3 g/L) for 1 hour and then stimulated with 300 μM hydrogen peroxide (H2O2) for 24 hours. The cells were randomly divided into the following groups: control, H2O2, H2O2+WXKL 1 g/L, and H2O2+WXKL 3 g/L groups.

2.2. Experimental Animals and Protocol

SD male rats aged 8 weeks (average body weight of ) were purchased from Beijing HuaFuKang Bioscience Co., Ltd. (Beijing, China). These rats were fed under controlled conditions with a constant temperature of , a humidity of , and a 12 h day/night cycle. All rats accepted normal chow diet of 1 week for acclimation before initiation of the study. All rats were assigned randomly to the following 3 groups by a random number table: control, DM, and DM+WXKL groups. These rats of a diabetic group, including DM and DM+WXKL groups, were fed with HFD (60 kcal% fat, 20 kcal% carbohydrate, and 20 kcal% protein; H10060, Beijing HuaFuKang Bioscience Co., Ltd., Beijing, China), while the control group was fed with normal chow diet throughout the whole study. After 4-week feeding, all animals were overnight fasted; then, the diabetic group was induced by a single tail vein injection of STZ (30 mg/kg; Sigma-Aldrich, St. Louis, MO, USA) in 0.1 M citrate buffer (pH 4.5). The rats in the control group were injected with the citrate buffer vehicle. 72 hours after injection, fasting blood glucose levels (FBG) were measured, and rats in the STZ injection group with blood glucose were considered diabetic models and would be used in future experiments. This model involves a combination of a diet high in fat to bring about hyperinsulinemia, insulin resistance, and/or glucose intolerance followed by treatment with the β-cell toxin STZ, which results in a severe reduction in functional β-cell mass [1921]. WXKL was kindly supplied by Shandong Buchang Pharmaceutical Co., Ltd. (Heze, China). The DM+WXKL group was given to the rats by daily lavage of WXKL (3 g/kg) dissolved in distilled water, and the other groups daily received distilled water only. We performed the following experiments on all rats after 8 weeks of treatment. Animal protocols adopted in the present study were approved by the Experimental Animal Administration Committee of Tianjin Medical University (Approval No. TMUaMEC2019004), which follows the guidelines established by the U.S. National Institutes of Health.

2.3. Mitochondrial Membrane Potential and ROS Measurement of Atrial Fibroblasts

The atrial fibroblasts were incubated with JC-1 staining buffer in the dark for 20 min at 37°C and washed twice with PBS without Ca2+ and Mg2+. The processes of measurement were used with Olympus FV1000 LSCM under excitation wavelength of 488 nm and 543 nm. The decreased relative fluorescence proportion of aggregate JC-1 (red)/monomeric JC-1 (green) indicates a decrease in the mitochondrial membrane potential (MMP). ROS were detected using the 2,7-dichlorofluorescin diacetate (DCFH-DA, Sigma-Aldrich) fluorescent probe. The cells were incubated with 10 μM DCFH-DA in PBS without Ca2+ and Mg2+ in the dark for 20 min at 37°C. Fluorescence was determined at 488 nm for excitation and 525 nm for emission. Microscope images were saved as TIFF files and processed for densitometric quantification with ImageJ version 1.46 (NIH). Software settings were kept the same for every image analyzed.

2.4. Assay of Cellar Mitochondrial Oxygen Consumption Rate

The mitochondrial oxygen consumption rate (OCR) of atrial fibroblasts was measured using the Seahorse Bioscience XF24 Extracellular Flux Analyzer (Seahorse Bioscience), and this process was according to instructions of the manufacturer and Lay et al. [22]. Briefly, atrial fibroblasts were cultured on a Seahorse XF microplate as required with an equal number per well and treated according to the protocol. The Seahorse XF24 extracellular flux assay plate was hydrated for 18 hours without CO2 in XF calibration buffer at 37°C before assay. 10 μM oligomycin, 10 μM carbonyl cyanide 4-(trifluoromethoxy) phenylhydrazone (FCCP), and 10 μM antimycin A (AA)+retenone were injected in turn during the process of assay.

2.5. Echocardiographic Assessments

After 8 weeks of treatment in each group, rats were allowed to inhale isoflurane (1.5 L/min) for anesthesia and placed on a 37°C thermal table in the supine position to measure transthoracic echocardiography. Echocardiographic parameters, including left atrial (LA) diameter (LAD), left ventricular posterior wall thickness (LVPWT), interventricular septal thickness (IVST), left ventricular end-diastolic dimension (LVEDD), and left ventricular end-systolic dimension (LVESD), were obtained in the parasternal long-axis view using a specified small animal ultrasound system (VisualSonics Vevo 2100, SONICS, Newtown, CT, USA) by a senior blinded operator. These parameters were measured by 2-dimensional imaging during 3 consecutive cardiac ejection cycles. Left ventricular ejection fraction (LVEF) was acquired in line with ventricular volumes calculated by the Teichholz formula:

2.6. Surface Electrocardiographic and Hemodynamic Experiment and Sample Collection

At the end of echocardiographic examination, each rat underwent right carotid artery cannulation allowing measurements of hemodynamic parameters using a Millar catheter during electrocardiographic (ECG) monitoring. Aortic systolic blood pressure (SBP), diastolic blood pressure (DBP), and mean blood pressure (MBP) were recorded carefully after a stabilization period. Subsequently, the cannula was inserted through the aortic valve to the left ventricle to record the left ventricular end-diastolic pressure (LVEDP) and maximum increasing or decreasing rate of left ventricular pressure (±dp/dt max). 10 stable waveforms of electrocardiogram were selected to measure heart rate, P wave duration, PR interval, QRS duration, and QT interval. Finally, rats were instantly euthanized. Then, blood samples were obtained from the right ventricle and LA tissues were rapidly separated. Samples for histological assessment were soaked in neutral buffered 10% formalin solution, and samples for molecular biological experiments were rapidly frozen in liquid nitrogen and stored at -80°C.

2.7. Serum Biochemical and Biomarker Measurements

FBG levels were detected with the blood glucose meter and test strips each week. Serum biochemical parameters including total cholesterol (TC), triglycerides (TG), low-density lipoprotein cholesterol (LDL-C), high-density lipoprotein cholesterol (HDL-C), and creatinine (Cr) level were detected using a fully automatic biochemical analyzer. Rat ELISA kits were used to detect the serum levels of insulin and high-sensitivity C-reactive protein (hs-CRP) (Wuhan Huamei Biological Engineering Co, Ltd., China); also, lipid peroxidation malondialdehyde (MDA) and superoxide dismutase (SOD) levels were measured according to instructions of the manufacturer (Nanjing Jiancheng Bioengineering Institute, China).

2.8. Electrophysiological Study

The rats were intraperitoneally injected with 3% pentobarbital sodium (50 mg/kg) for anesthesia. The heart was quickly isolated and placed in 4°C Tyrode’s solution to wash out residual blood and to remove residual lung tissue. Then, the aorta was cannulated and connected to a Langendorff perfusion system. The Langendorff perfusion system was filled with 37°C Tyrode’s solution equilibrated with 5% CO2 and 95% O2. Preperfusion was performed for 20 minutes to minimize endogenous release of catecholamine residual effects. Some hearts could not maintain normal rhythms after 20 minutes and were abandoned.

Epicardial activating electrical mapping was recorded by a electrode microelectrode (electrode impedance: 1.5-1.7Q, PA03606060101, multielectrode probe array) on the epicardial surface of the left and right atrium. Data were recorded by multichannel systems (EMS64-USB-1003, United Kingdom). Activation waveforms acquired were amplified by a filter amplifier and thereby transmitted to the connected computer. All activation time was digitized and then used to draw activation maps. The activation times were calculated as the point of maximal negative slope of activation waveforms. Conduction velocity (CV), inhomogeneity index, and absolute inhomogeneity were calculated by EMapScope 4.0 software (MappingLab Ltd., UK).

Three silver bipolar electrodes were placed on the left atrium, right atrium, and right ventricular apex after recorded epical mapping, and the entire recorded process was connected to a custom-made computer software program (Electrophysiological Recording System, TOP-2001, HTONG Company, Shanghai, China). There were 3 basic cycle lengths (BCLs) of basic stimuli (S1), including 200 ms, 150 ms, and 100 ms. When the sinus cycle length (SCL) was shorter than 200 ms, we used the SCL subtracted by 10 ms to replace BCL of 200 ms. The interatrial conduction time (IACT) was measured during right atrium pacing. Then, atrial-ventricular Wenckebach cycle length conduction (AVWCL) was measured by right atrial (RA) incremental pacing. The S1S1 interval was decreased in 5 ms steps until ventricular rhythm was not 1 : 1 following atrial pacing. 8 S1 were followed by a premature extra stimulus (S2) to measure the atrial effective refractory period (ERP). The S1S2 interval was decreased in 2 ms steps until the longest S1S2 interval that failed to capture the depolarization. The stimulation order of burst pacing was from the right atrium to the left atrium. AF induction was verified by burst pacing (cycle lengths of 50 ms, 40 ms, and 30 ms) for 3 seconds, respectively, which was performed 5 times with 30-second intervals. AF was defined as rapid, irregular atrial response longer than 1 second. AF inducibility was defined as the percentage of burst pacing leading to AF episodes.

2.9. Isolation of Atrial Mitochondria and Measurement of Atrial MMP

Rats were euthanized with 3% pentobarbital sodium (50 mg/kg), and median sternotomy was immediately performed. The LA mitochondria were isolated, and the mitochondrial protein content was assayed according to our previous studies. Atrial MMP was assessed by JC-1 staining (Beyotime, Jiangsu, China). 300 μg of mitochondrial protein in 2 mL of respiration medium were incubated with JC-1 working solution at 37°C in the dark for 10 min.

2.10. Western Blot Analysis

Frozen LA tissues were homogenized in liquid nitrogen, and the total protein was extracted by RIPA lysis buffer. The lysates were centrifuged at 15,000g for 20 minutes, and the supernatants were collected. Protein concentrations were measured by the bicinchoninic acid (BCA) protein assay regent kit (Thermo Scientific, USA). All sample proteins loaded equally with 60 μg were separated by sodium dodecyl sulfate-polyacrylamide gel electrophoresis (SDS-PAGE) and transferred by electrophoresis to a polyvinylidene difluoride (PVDF) membrane. Subsequently, PVDF membranes were blocked for 1 h with 5% nonfat dry milk or bovine serum albumin (BSA) in Tris-buffered saline containing 0.1% Tween 20 (TBST), then incubated at 4°C overnight with a primary antibody. Then, the membrane was washed with TBST and incubated with the horseradish peroxidase-conjugated secondary antibody for 1 hour. The primary antibodies used were as follows: β-actin (1 : 5000, 60008-1-Ig, Proteintech), mitochondrial transcription factor A (TFAM, 1 : 2000, ab131607, Abcam), dynamin-related protein (Drp1, 1 : 1000, ab5678, Abcam), mitofusin 2 (Mfn2, 1 : 1000, ab56889, Abcam), transforming growth factor-β (TGF-β, 1 : 1000, ab190503, Abcam), nuclear factor kappa-b (NF-κb, 1 : 1000, ab90532, Abcam), Bcl-2 (1 : 1000, ab59348, Abcam), Bax (1 : 5000, ab32503, Abcam), collagen I (1 : 1000, ab34710, Abcam), collagen III (1 : 5000, ab7778, Abcam), and α-smooth muscle actin (α-SMA, 1 : 5000, ab5694, Abcam). β-Actin was evaluated as a loading control. The reactions were visualized using Tanon 5200 Multi Chemiluminescent Imaging System (Tanon Science & Technology Co., Ltd., Shanghai, China).

2.11. Histological Studies

The tissues were cut into 5 μm cross sections, then stained with hematoxylin and eosin (HE) to observe the morphological changes and Masson’s trichrome stain to evaluate interstitial fibrosis. Digital images were scanned by Image-Pro Plus 6.0, and the extent of fibrosis was determined by dividing the area of collagen deposition by the entire cardiac tissue area. Five randomly selected sections of each group were utilized for quantification. The cardiac collagen volume fraction and cross-sectional area were analyzed using SPSS 17.0.

2.12. Statistical Analysis

Data were presented as (SD). Differences between the groups were analyzed for statistical significance using the one-way analysis of variance (ANOVA) followed by the Least Significant Difference (LSD) test. All data were analyzed using SPSS 17.0, and values < 0.05 were considered significantly altered.

3. Results

3.1. WXKL Decreases ROS and Improves Mitochondrial Function of Atrial Fibroblasts

DCFH-DA fluorescence was measured in atrial fibroblasts from each experimental group (Figure 1(a)). ROS was significantly higher in the H2O2 group compared with the control group ( vs. , , Figure 1(b)). The concentration of WXKL used in our previous clinical study was doubled, which was used in clinical practice. In this in vitro cell experiment, we compared doubled concentration (1 g/L) and six-fold concentration (3 g/L) of WXKL. The ROS level in the H2O2+WXKL 1 g/L group and the H2O2+WXKL 3 g/L group was and , respectively (Figure 1(b)). The ROS was markedly decreased in the H2O2+WXKL 3 g/L group (), while ROS already had a decreased trend in the H2O2+WXKL 1 g/L group () compared with the H2O2 group.

OCR measurements then permitted us to investigate whether WXKL improved mitochondrial function. Basal respiration and maximal respiration were also decreased in the H2O2 group compared with the control group, and the above changes were improved in the H2O2+WXKL 3 g/L group (Figure 1(c)). There were no differences of ATP production and nonmitochondrial respiration in all groups (Figure 1(c)). MMP was quantified using the JC-1 dye (Figure 1(d)). The MMP was significantly reduced in the H2O2 group (, ). The MMP was similar between the H2O2 group and the H2O2+WXKL 1 g/L group (Figure 1(e)). And the MMP was improved in H2O2+WXKL 3 g/L.

3.2. WXKL Improves Left Atrial MMP in Type 2 Diabetic Rats

We successfully established a rat model of type 2 diabetes by high-fat feeding+low STZ injection. FBG was stabilized in a hyperglycemic state within 8 weeks of the whole study process. The general characteristics of the 3 groups are presented in Table 1. Thus, after four weeks of high-fat diet, FBG was slightly elevated in the DM group (, ) and DM+WXKL group (, ) compared with the control group (), and there was no difference in FBG between the two diabetic groups (). Blood glucose was significantly higher in the DM (, ) and DM+WXKL groups (, ) compared with the control group (). Serum insulin level, quantified by ELISA, was significantly higher in the DM () and DM+WXKL groups () when compared to the control group ().

Control group ()DM group ()DM+WXKL group () value

Weight (g)0.012
Heart weight ratio (1/1000)0.009
Blood glucose (mmol/L)<0.001
IVS (mm)0.337
LVPW (mm)0.213
Insulin (pmol/L)0.006
hs-CRP (mg/L)0.017
SOD (U/mL)#0.030
MDA (nmol/L)##<0.001
BUN (mmol/L)0.324
Cr (μmol/L)0.724
HDL-c (mmol/L)0.567
LDL-c (mmol/L)0.275
TC (mmol/L)0.003
TG (mmol/L)0.012

Values are expressed as . DM = diabetes mellitus; WXKL = Wenxin Keli; IVS = interventricular septum; LVPW = left ventricular posterior wall; hs-CRP = high-sensitivity C-reactive protein; SOD = superoxide dismutase; MDA = malondialdehyde; BUN = blood urea nitrogen; Cr = creatinine; HDL-c = high-density lipoprotein cholesterol; LDL-c = low-density lipoprotein cholesterol; TC = cholesterol; TG = triglyceride. Compared with the control group, . Compared with the control group, . #Compared with the DM group, ##Compared with the DM group, .

After 8 weeks of WXKL administration, mitochondria of the left atrium were extracted for MMP detection (Figure 1(f)). MMP was decreased in the DM group compared with the control group ( vs. , ). The MMP of the DM+WXKL group was also lower than that of the control group ( vs. , ). However, the MMP of the DM+WXKL group was improved compared with that of the DM group ( vs. , ).

3.3. WXKL Improves Atrial Remodeling and Prevents Atrial Fibrillation

Representative echocardiographic images of the three groups are shown in Figure 2(a). We found that LAD increased in the DM group compared with the control group ( vs. , , Figure 2(b)). LAD in the DM+WXKL and DM groups were not significantly different ( vs. , ). There were no differences in LVEF, IVS, and LVPW between the three groups (Figure 2(c) and Table 1). For ECG data, P wave duration, PR interval, and QRS duration were not significantly different between the three experimental groups (Figure 2(d)).

We measured hemodynamics through a Miller pressure catheter. SBP, DBP, and MBP were not significantly different between the three groups (Figure 2(e)). However, +dp/dt and -dp/dt in the DM group were significantly lower than those in the control group ( vs. () and vs. (), Figure 2(f)). The above parameters were improved in the DM+WXKL group. There was no difference of LVEDP between the three groups (Figure 2(g)).

Electrophysiological parameters were obtained from Langendorff-perfused hearts. We firstly recorded electrical conduction mapping of LA (Figure 3(a)) and RA (Figure 3(e)). Mapping images showed that left atrial conduction velocity (LACV) was significantly lower in the DM group than in the control group ( vs. , , Figure 3(b)). This was significantly improved in the DM+WXKL group ( vs. , , Figure 3(b)). LA conduction dispersion was higher in the DM group than in the control group (absolute vs. , index vs. , ; Figures 3(c) and 3(d)). LA conduction dispersion of the DM+WXKL group was reduced compared with that of the DM group. LA electrical conductions of the control group were uniform and showed an orderly spread to the surrounding tissue. However, LA conduction of the DM group was disordered and there were abnormal conduction positions in the wave conduction, but it was restored in the DM+WXKL group. Comparable results were observed in the mapping images of RA electrical conduction maps (Figures 3(e) and 3(f)3(h)).

There were no significant differences of SCL and AVWCL between the three groups (Figure 3(i)). The IACT of the DM group was slightly longer than that of the control group in 200 ms and 150 ms of BCL (Figure 3(j)). We also measured RAERP and LAERP in all three BCLs (Figures 3(k) and 3(l)). RAERP and LAERP in the three groups were also statistically indistinguishable. A representative AF episode induced by LA burst pacing is shown in Figure 3(m). We observed that the AF incidence was significantly higher in the DM group than in the control group (50.94% vs. 18.12%, , Figure 3(n)). The AF incidence in the DM+WXKL group was considerably lower than that in the DM group (19.06% vs. 50.94%, , Figure 3(n)). Meanwhile, there was no significant difference between the DM+WXKL group and the control group ().

H&E and Masson’s trichrome staining was used to detect morphological changes in the RA (Figure 4(a)). Cardiomyocytes in the control group had normal morphology, but its cross-sectional area was higher in the DM group (Figure 4(b)). The ratio of myocardial interstitial fibrosis was higher in the DM group compared with the control group ( vs. , , Figure 4(c)). However, cardiomyocyte hypertrophy and fibrosis ratio were alleviated in the DM+WXKL group.

3.4. WXKL Improves Serum Oxidative Stress

Different serum biomarkers were measured. hs-CRP levels were higher in the DM group and DM+WXKL group than in the control group (Table 1). There was no difference between the DM group and the DM+WXKL group ( vs. , ). Lower SOD and higher MDA levels were detected in the DM group compared to the control group (Table 1). Serum levels of BUN, Cr, HDL-C, and LDL-C were not significantly different amongst the three groups (Table 1). Meanwhile, TC and TG were significantly higher in the DM group than in the control group, and these markers could not be aggravated by WXKL treatment (Table 1).

3.5. WXKL Upregulates Mitochondria-Associated Proteins and Reduces Apoptosis

We firstly evaluated the expression of mitochondria-associated protein of LA tissue and found that the expression levels of TFAM, Drp1, and Mfn2 were significantly lower in the DM group compared with the control group (Figures 5(a)5(c)). Encouragingly, expression levels of these mitochondria-associated proteins were significantly increased in the DM+WXKL group. We compared the expression levels of inflammatory proteins. TGF-β and NF-κb were upregulated in the DM group (Figures 5(d) and 5(e)). However, the expression levels of two inflammatory proteins were not different between the DM+WXKL group and DM group. Compared with the control group, the expressions of fibrotic proteins, collagen I, collagen III, and α-SMA, were significantly increased in the DM group (Figures 5(f)5(h)). These changes were significantly reversed in the DM+WXKL group.

Finally, we compared the apoptotic proteins between the three groups. It was found that the expression level of Bax was upregulated and the antiapoptotic protein Bcl-2 was downregulated in the DM group (Figure 5(i)). The expression levels of Bax and Bcl-2 were improved in the DM+WXKL group compared with the DM group and approached the expression level of the control group.

4. Discussion

In this study, we found that WXKL enhances mitochondrial function with improved basal and maximal respiration and reduces ROS production. WXKL treatment improved atrial remodeling and prevented AF by restoring mitochondrial function in diabetic rats.

DM is a well-recognized risk factor for the development of AF [4, 2325]. The results of serum markers showed that there were abnormal changes in inflammation and oxidative stress levels in diabetic rats, which is consistent with our previous studies [2628]. Mitochondrial dysfunction and molecular mechanisms underlying DM-related AF development have been reported [10, 24]. ROS is a critical factor mediating both DM and AF [5, 24, 29]. A variety of sources, including NADPH oxidase [26], mitochondrial enzymes [28], and xanthine oxidase [27], generate ROS in the context of AF [30, 31]. Mitochondria-derived ROS are considered the main ROS source of age-related AF [32]. Therefore, mitochondrial oxidative stress is a potential target [24].

Mitochondrial homeostasis is important for maintaining the normal function of mitochondria [33, 34]. Patients with T2DM and obesity demonstrated reduced expression of Mfn2, which may be related to the reduced function of mitochondria [35]. Excessive mitochondrial fission or slowing mitochondrial fusion leads to an increase in mitochondrial fragmentation [36]. A decreasing mitochondrial volume accelerates the speed of the electron transport chain. However, a reduced mitochondrial inner membrane area makes mitochondria susceptible to calcium overload, which initiates apoptosis [36]. Mfn2-deficient mice display enlarged cardiomyocytes and modest cardiac hypertrophy with functional deterioration [37]. Hence, the expression levels of mitochondria-related proteins were decreased in the DM group to reflect abnormal mitochondrial function. Bax is required for the physiological fusion of mitochondria from elongated mitochondria via the functional activity of outer mitochondrial membrane (OMM) proteins including Mfn2, which inhibit cytochrome c release [38]. The treatment effect of WXKL improved on these proteins.

blockers including ranolazine and WXKL can effectively suppress AF [15, 16, 39]. blockade of WXKL is atrial-selective in animal coronary perfused atrial preparations at concentrations that cause no effect in the ventricles [13]. Hu et al. suggested that this character of WXKL is due to more negative steady-state inactivation, less negative resting membrane potential, and shorter diastolic intervals in atrial cells [13]. Ranolazine can maintain mitochondrial function and reduce mitochondrial ROS levels in cardiac disorders [40]. The protection of ranolazine against AF development is due to inhibition of late sodium current (), reducing intracellular calcium overload [41, 42]. We also found that in DM, MMP of the atrial myocardium is significantly decreased but this was improved by WXKL treatment. These findings are consistent with the preservation of mitochondrial respiration. The effects of WXKL and ranolazine on mitochondria may be similar.

Our research was aimed at clarifying the signaling pathway of WXKL intervention. H2O2 treatment occurred with the outbreak of ROS, which was related to the change of mitochondria (opening of mitochondrial permeability transition pore and decrease in MMP). H2O2 can diffuse across the membrane and generate other ROS. Superoxide released into the mitochondrial matrix can react with mitochondrial DNA (mtDNA), and ROS-induced mtDNA damage leads to respiratory complex enzyme dysfunction [43]. H2O2 delivered to the cytoplasm is involved in a variety of signaling pathways, including mitogen-activated protein kinase (MAPK), c-Jun N-terminal kinase (JNK1), and TNF-α/NF-κb [4446]. Through the activation of these signaling pathways, the mitochondrial dysfunction of atrial fibroblasts led to collagen production and myofibroblast differentiation, decreased cell viability, and increased apoptosis [18]. We demonstrated that WXKL improved mitochondrial function in vitro. Therefore, WXKL can regulate the activation of the signaling pathway induced by H2O2 to prevent profibrotic cellular activities. Low concentrations of WXKL inhibit and suppress acetylcholine-induced AF, while higher concentrations inhibit fast sodium current and prevent ventricular reentrant arrhythmias. It exerts a tonic block on peak without significant use dependence and interacts with its inactivated state [13]. WXKL binds to the inactivated state of peak and dissociates rapidly. WXKL is speculated to possess antisinus arrhythmia, antiheart failure, and antihypertensive properties [47]. The mechanism of WXKL for mitochondrial function still needs validation in future work.

Several limitations of our study should be noted. Firstly, we did not block the pathway of mitochondrial oxidation in vitro, and we could not further clarify that ROS was a sole signaling pathway to improve mitochondrial function by WXKL. OCR of atrial fibroblasts was used as a marker of mitochondrial function. Secondly, we only assessed the effects of WXKL in atrial fibroblasts, and potential effects of WXKL on atrial cardiomyocytes were not investigated. Thirdly, ion channel currents of WXKL intervention were not studied in this study. Moreover, detailed electrophysiological mechanisms of the antiarrhythmic effects of WXKL, such as alterations in autonomic tone, calcium handling, and depolarization and repolarization dynamics, remain to be elucidated. In addition, action morphology will be measured in the presence and absence of WXKL in single atrial myocytes isolated from normal and diabetic hearts. WXKL may have non-DM-related biological effects in control rats. Further studies need to detail all the mechanisms of WXKL on the atrium by regulating the DM-induced mitochondrial oxidative stress.

5. Conclusion

WXKL can inhibit oxidative stress and improve mitochondrial function in vitro induced by H2O2 and in vivo induced by DM, alleviate atrial remodeling, and reduce AF incidence in DM rats.

Data Availability

The data used to support the findings of this study are available from the corresponding author upon request.

Conflicts of Interest

The authors have no conflicts of interest to declare.

Authors’ Contributions

Mengqi Gong and Ming Yuan are the first two authors who contributed equally to this work.


This work was supported by grants from the National Natural Science Foundation of China (grant nos. 81970270 and 81570298 to T.L.) and Tianjin Natural Science Foundation (grant no. 16JCZDJC34900 to T.L.).

Supplementary Materials

Appendix Figure 1: representative atrial fibrillation episodes induced by right atrium (RA) burst pacing. LA: left atrium; RV: right ventricle. Appendix Figure 2: the representative image of hemodynamic data from a Millar catheter. LVEDP: left ventricular end-diastolic pressure; ECG: electrocardiographic. Appendix Figure 3: all western blot results of transcription factor A (TFAM). Appendix Figure 4: all western blot results of dynamin-related protein 1 (Drp1). Appendix Figure 5: all western blot results of mitofusin 2 (Mfn2). Appendix Figure 6: all western blot results of transforming growth factor-β (TGF-β). Appendix Figure 7: all western blot results of nuclear factor kappa-b (NF-κb). Appendix Figure 8: all western blot results of α-smooth muscle actin (α-SMA). Appendix Figure 9: all western blot results of collagen I. Appendix Figure 10: all western blot results of collagen III. Appendix Figure 11: all western blot results of Bcl-2. Appendix Figure 12: all western blot results of Bax. (Supplementary Materials)


  1. A. Odutayo, C. X. Wong, A. J. Hsiao, S. Hopewell, D. G. Altman, and C. A. Emdin, “Atrial fibrillation and risks of cardiovascular disease, renal disease, and death: systematic review and meta-analysis,” British Medical Journal, vol. 354, article i4482, 2016. View at: Publisher Site | Google Scholar
  2. D. Conen, C. U. Chae, R. J. Glynn et al., “Risk of death and cardiovascular events in initially healthy women with new-onset atrial fibrillation,” JAMA, vol. 305, no. 20, pp. 2080–2087, 2011. View at: Publisher Site | Google Scholar
  3. L. Staerk, J. A. Sherer, D. Ko, E. J. Benjamin, and R. H. Helm, “Atrial fibrillation: epidemiology, pathophysiology, and clinical outcomes,” Circulation Research, vol. 120, no. 9, pp. 1501–1517, 2017. View at: Publisher Site | Google Scholar
  4. E. J. Benjamin, P. Muntner, A. Alonso et al., “Heart disease and stroke statistics-2019 update: a report from the American Heart Association,” Circulation, vol. 139, no. 10, pp. e56–e528, 2019. View at: Publisher Site | Google Scholar
  5. A. Wang, J. B. Green, J. L. Halperin, and J. P. Piccini Sr., “Atrial fibrillation and diabetes mellitus: JACC review topic of the week,” Journal of the American College of Cardiology, vol. 74, no. 8, pp. 1107–1115, 2019. View at: Publisher Site | Google Scholar
  6. H. Fu, G. Li, C. Liu et al., “Probucol prevents atrial remodeling by inhibiting oxidative stress and TNF-α/NF-κB/TGF-β signal transduction pathway in alloxan-induced diabetic rabbits,” Journal of Cardiovascular Electrophysiology, vol. 26, no. 2, pp. 211–222, 2015. View at: Publisher Site | Google Scholar
  7. R. B. Neuman, H. L. Bloom, I. Shukrullah et al., “Oxidative stress markers are associated with persistent atrial fibrillation,” Clinical Chemistry, vol. 53, no. 9, pp. 1652–1657, 2007. View at: Publisher Site | Google Scholar
  8. A. Bukowska, L. Schild, G. Keilhoff et al., “Mitochondrial dysfunction and redox signaling in atrial tachyarrhythmia,” Experimental Biology and Medicine, vol. 233, no. 5, pp. 558–574, 2008. View at: Publisher Site | Google Scholar
  9. U. Lendeckel, C. Müller, C. Röcken et al., “Expression of opioid receptor subtypes and their ligands in fibrillating human atria,” Pacing and Clinical Electrophysiology, vol. 28, Supplement 1, pp. S275–S279, 2005. View at: Publisher Site | Google Scholar
  10. D. Montaigne, X. Marechal, P. Lefebvre et al., “Mitochondrial dysfunction as an arrhythmogenic substrate: a translational proof-of-concept study in patients with metabolic syndrome in whom post-operative atrial fibrillation develops,” Journal of the American College of Cardiology, vol. 62, no. 16, pp. 1466–1473, 2013. View at: Publisher Site | Google Scholar
  11. X. Xue, D. Guo, H. Sun et al., “Wenxin Keli suppresses ventricular triggered arrhythmias via selective inhibition of late sodium current,” Pacing and Clinical Electrophysiology, vol. 36, no. 6, pp. 732–740, 2013. View at: Publisher Site | Google Scholar
  12. A. Burashnikov, A. Petroski, D. Hu, H. Barajas-Martinez, and C. Antzelevitch, “Atrial-selective inhibition of sodium-channel current by Wenxin Keli is effective in suppressing atrial fibrillation,” Heart Rhythm, vol. 9, no. 1, pp. 125–131, 2012. View at: Publisher Site | Google Scholar
  13. D. Hu, H. Barajas-Martínez, A. Burashnikov, B. K. Panama, J. M. Cordeiro, and C. Antzelevitch, “Mechanisms underlying atrial-selective block of sodium channels by Wenxin Keli: experimental and theoretical analysis,” International Journal of Cardiology, vol. 207, pp. 326–334, 2016. View at: Publisher Site | Google Scholar
  14. A. Burashnikov, J. M. Di Diego, A. C. Zygmunt, L. Belardinelli, and C. Antzelevitch, “Atrium-selective sodium channel block as a strategy for suppression of atrial fibrillation: differences in sodium channel inactivation between atria and ventricles and the role of ranolazine,” Circulation, vol. 116, no. 13, pp. 1449–1457, 2007. View at: Publisher Site | Google Scholar
  15. N. Zhang, G. Tse, S. Dahal et al., “Efficacy of Wenxin Keli plus amiodarone versus amiodarone monotherapy in treating recent-onset atrial fibrillation,” Cardiology Research and Practice, vol. 2018, Article ID 6047271, 7 pages, 2018. View at: Publisher Site | Google Scholar
  16. Z. Meng, J. Tan, Q. He et al., “Wenxin Keli versus sotalol for paroxysmal atrial fibrillation caused by hyperthyroidism: a prospective, open label, and randomized study,” Evidence-based Complementary and Alternative Medicine, vol. 2015, Article ID 101904, 9 pages, 2015. View at: Publisher Site | Google Scholar
  17. D. K. Yang and S. J. Kim, “Cucurbitacin I protects H9c2 cardiomyoblasts against H2O2-induced oxidative stress via protection of mitochondrial dysfunction,” Oxidative Medicine and Cellular Longevity, vol. 2018, Article ID 3016382, 11 pages, 2018. View at: Publisher Site | Google Scholar
  18. M. Singh, H. Sharma, and N. Singh, “Hydrogen peroxide induces apoptosis in HeLa cells through mitochondrial pathway,” Mitochondrion, vol. 7, no. 6, pp. 367–373, 2007. View at: Publisher Site | Google Scholar
  19. S. Skovso, “Modeling type 2 diabetes in rats using high fat diet and streptozotocin,” Journal of Diabetes Investigation, vol. 5, no. 4, pp. 349–358, 2014. View at: Publisher Site | Google Scholar
  20. P. J. Antony, G. R. Gandhi, A. Stalin et al., “Myoinositol ameliorates high-fat diet and streptozotocin-induced diabetes in rats through promoting insulin receptor signaling,” Biomedicine & Pharmacotherapy, vol. 88, pp. 1098–1113, 2017. View at: Publisher Site | Google Scholar
  21. A. F. Aydın, İ. Bingül, C. Küçükgergin, I. Doğan-Ekici, S. Doğru Abbasoğlu, and M. Uysal, “Carnosine decreased oxidation and glycation products in serum and liver of high-fat diet and low-dose streptozotocin-induced diabetic rats,” International Journal of Experimental Pathology, vol. 98, no. 5, pp. 278–288, 2017. View at: Publisher Site | Google Scholar
  22. S. Lay, O. Sanislav, S. J. Annesley, and P. R. Fisher, “Mitochondrial stress tests using seahorse respirometry on intact Dictyostelium discoideum cells,” Methods in Molecular Biology, vol. 1407, no. 4, pp. 41–61, 2016. View at: Publisher Site | Google Scholar
  23. E. J. Benjamin, D. Levy, S. M. Vaziri, R. B. D'Agostino, A. J. Belanger, and P. A. Wolf, “Independent risk factors for atrial fibrillation in a population-based cohort: The Framingham Heart Study,” JAMA, vol. 271, no. 11, pp. 840–844, 1994. View at: Publisher Site | Google Scholar
  24. A. Faria and S. J. Persaud, “Cardiac oxidative stress in diabetes: mechanisms and therapeutic potential,” Pharmacology & Therapeutics, vol. 172, pp. 50–62, 2017. View at: Publisher Site | Google Scholar
  25. I. Russo and N. G. Frangogiannis, “Diabetes-associated cardiac fibrosis: cellular effectors, molecular mechanisms and therapeutic opportunities,” Journal of Molecular and Cellular Cardiology, vol. 90, pp. 84–93, 2016. View at: Publisher Site | Google Scholar
  26. J. Qiu, J. Zhao, J. Li et al., “NADPH oxidase inhibitor apocynin prevents atrial remodeling in alloxan-induced diabetic rabbits,” International Journal of Cardiology, vol. 221, pp. 812–819, 2016. View at: Publisher Site | Google Scholar
  27. Y. Yang, J. Zhao, J. Qiu et al., “Xanthine oxidase inhibitor allopurinol prevents oxidative stress-mediated atrial remodeling in alloxan-induced diabetes mellitus rabbits,” Journal of the American Heart Association, vol. 7, no. 10, article e008807, 2018. View at: Publisher Site | Google Scholar
  28. X. Zhang, Z. Zhang, Y. Zhao et al., “Alogliptin, a dipeptidyl peptidase-4 inhibitor, alleviates atrial remodeling and improves mitochondrial function and biogenesis in diabetic rabbits,” Journal of the American Heart Association, vol. 6, no. 5, article e005945, 2017. View at: Publisher Site | Google Scholar
  29. Y. Guo, G. Y. Lip, and S. Apostolakis, “Inflammation in atrial fibrillation,” Journal of the American College of Cardiology, vol. 60, no. 22, pp. 2263–2270, 2012. View at: Publisher Site | Google Scholar
  30. A. A. Sovari and S. C. Dudley Jr., “Reactive oxygen species-targeted therapeutic interventions for atrial fibrillation,” Frontiers in Physiology, vol. 3, article 311, 2012. View at: Publisher Site | Google Scholar
  31. C. Wolke, A. Bukowska, A. Goette, and U. Lendeckel, “Redox control of cardiac remodeling in atrial fibrillation,” Biochimica et Biophysica Acta, vol. 1850, no. 8, pp. 1555–1565, 2015. View at: Publisher Site | Google Scholar
  32. W. Xie, G. Santulli, S. R. Reiken et al., “Mitochondrial oxidative stress promotes atrial fibrillation,” Scientific Reports, vol. 5, no. 1, article 11427, 2015. View at: Publisher Site | Google Scholar
  33. C. Lopez-Crisosto, C. Pennanen, C. Vasquez-Trincado et al., “Sarcoplasmic reticulum-mitochondria communication in cardiovascular pathophysiology,” Nature Reviews Cardiology, vol. 14, no. 6, pp. 342–360, 2017. View at: Publisher Site | Google Scholar
  34. M. N. Serasinghe and J. E. Chipuk, “Mitochondrial fission in human diseases,” Handbook of Experimental Pharmacology, vol. 240, pp. 159–188, 2017. View at: Publisher Site | Google Scholar
  35. C. E. Fealy, A. Mulya, N. Lai, and J. P. Kirwan, “Exercise training decreases activation of the mitochondrial fission protein dynamin-related protein-1 in insulin-resistant human skeletal muscle,” Journal of Applied Physiology (Bethesda, Md. : 1985), vol. 117, no. 3, pp. 239–245, 2014. View at: Publisher Site | Google Scholar
  36. M. Liesa and O. S. Shirihai, “Mitochondrial dynamics in the regulation of nutrient utilization and energy expenditure,” Cell Metabolism, vol. 17, no. 4, pp. 491–506, 2013. View at: Publisher Site | Google Scholar
  37. K. N. Papanicolaou, M. M. Phillippo, and K. Walsh, “Mitofusins and the mitochondrial permeability transition: the potential downside of mitochondrial fusion,” American Journal of Physiology - Heart and Circulatory Physiology, vol. 303, no. 3, pp. H243–H255, 2012. View at: Publisher Site | Google Scholar
  38. R. Sugioka, S. Shimizu, and Y. Tsujimoto, “Fzo1, a protein involved in mitochondrial fusion, inhibits apoptosis,” Journal of Biological Chemistry, vol. 279, no. 50, pp. 52726–52734, 2004. View at: Publisher Site | Google Scholar
  39. M. Gong, Z. Zhang, N. Fragakis et al., “Role of ranolazine in the prevention and treatment of atrial fibrillation: a meta-analysis of randomized clinical trials,” Heart Rhythm, vol. 14, no. 1, pp. 3–11, 2017. View at: Publisher Site | Google Scholar
  40. D. Zou, N. Geng, Y. Chen et al., “Ranolazine improves oxidative stress and mitochondrial function in the atrium of acetylcholine-CaCl2 induced atrial fibrillation rats,” Life Sciences, vol. 156, pp. 7–14, 2016. View at: Publisher Site | Google Scholar
  41. M. Aldakkak, A. K. Camara, J. S. Heisner, M. Yang, and D. F. Stowe, “Ranolazine reduces Ca2+ overload and oxidative stress and improves mitochondrial integrity to protect against ischemia reperfusion injury in isolated hearts,” Pharmacological Research, vol. 64, no. 4, pp. 381–392, 2011. View at: Publisher Site | Google Scholar
  42. F. Corradi, L. Paolini, and R. De Caterina, “Ranolazine in the prevention of anthracycline cardiotoxicity,” Pharmacological Research, vol. 79, pp. 88–102, 2014. View at: Publisher Site | Google Scholar
  43. M. P. Murphy, “How mitochondria produce reactive oxygen species,” Biochemical Journal, vol. 417, no. 1, pp. 1–13, 2009. View at: Publisher Site | Google Scholar
  44. E. Cadenas, “Mitochondrial free radical production and cell signaling,” Molecular Aspects of Medicine, vol. 25, no. 1-2, pp. 17–26, 2004. View at: Publisher Site | Google Scholar
  45. S. Nemoto, K. Takeda, Z. X. Yu, V. J. Ferrans, and T. Finkel, “Role for mitochondrial oxidants as regulators of cellular metabolism,” Molecular and Cellular Biology, vol. 20, no. 19, pp. 7311–7318, 2000. View at: Publisher Site | Google Scholar
  46. N. Suematsu, H. Tsutsui, J. Wen et al., “Oxidative stress mediates tumor necrosis factor-alpha-induced mitochondrial DNA damage and dysfunction in cardiac myocytes,” Circulation, vol. 107, no. 10, pp. 1418–1423, 2003. View at: Publisher Site | Google Scholar
  47. T. Wang, M. Lu, Q. du et al., “An integrated anti-arrhythmic target network of compound Chinese medicine Wenxin Keli revealed by combined machine learning and molecular pathway analysis,” Molecular BioSystems, vol. 13, no. 5, pp. 1018–1030, 2017. View at: Publisher Site | Google Scholar

Copyright © 2020 Mengqi Gong et al. This is an open access article distributed under the Creative Commons Attribution License, which permits unrestricted use, distribution, and reproduction in any medium, provided the original work is properly cited.

20 Views | 46 Downloads | 0 Citations
 PDF  Download Citation  Citation
 Download other formatsMore
 Order printed copiesOrder