Andrographolide inhibits arrhythmias and is cardioprotective in rabbits
Metrics: PDF 992 views | HTML 1767 views | ?
Mengliu Zeng1,*, Wanzhen Jiang1,*, Youjia Tian1, Jie Hao1, Zhenzhen Cao1, Zhipei Liu1, Chen Fu1, Peihua Zhang1 and Jihua Ma1
1Cardio-Electrophysiological Research Laboratory, Medical College of Wuhan University of Science and Technology, Wuhan, Hubei, China
*These authors have contributed equally to this work
Jihua Ma, email: firstname.lastname@example.org
Keywords: andrographolide, sodium current, L-type calcium current, action potential, arrhythmia
Received: January 17, 2017 Accepted: April 21, 2017 Published: May 22, 2017
Andrographolide has a protective effect on the cardiovascular system. To study its cardic-electrophysiological effects, action potentials and voltage-gated Na+ (INa), Ca2+ (ICaL), and K+ (IK1, IKr, Ito and IKur) currents were recorded using whole-cell patch clamp and current clamp techniques. Additionally, the effects of andrographolide on aconitine-induced arrhythmias were assessed on electrocardiograms in vivo. We found that andrographolide shortened action potential duration and reduced maximum upstroke velocity in rabbit left ventricular and left atrial myocytes. Andrographolide attenuated rate-dependence of action potential duration, and reduced or abolished delayed afterdepolarizations and triggered activities induced by isoproterenol (1 μM) and high calcium ([Ca2+]o=3.6 mM) in left ventricular myocytes. Andrographolide also concentration-dependently inhibited INa and ICaL, but had no effect on Ito, IKur, IK1, or IKr in rabbit left ventricular and left atrial myocytes. Andrographolide treatment increased the time and dosage thresholds of aconitine-induced arrhythmias, and reduced arrhythmia incidence and mortality in rabbits. Our results indicate that andrographolide inhibits cellular arrhythmias (delayed afterdepolarizations and triggered activities) and aconitine-induced arrhythmias in vivo, and these effects result from INa and ICaL inhibition. Andrographolide may be useful as a class I and IV antiarrhythmic therapeutic.
The traditional medical herb, Andrographis paniculata (Burm.f.) Wall. ex Nees, has been used for centuries to treat a variety of diseases in China. Andrographolide, its major bioactive component, has many pharmacological effects, including antitumor [1, 2], anti-inflammatory [1–4], antiviral , anti-hypertension , antioxidant [3, 6, 7], antihyperglycaemic , hepatoprotective [2, 7], and cardioprotective properties [5–11]. Recent studies found that andrographolide protected rat cardiomyocytes against hypoxia/reoxygenation injury by upregulating cellular-reduced glutathione levels and antioxidant enzyme activities . Andrographolide protected mouse hearts from LPS-induced cardiac malfunctions, and thus may prevent myocardial malfunction during sepsis . Because platelet activation is closely linked to coronary heart disease, andrographolide could be used to treat patients with thromboembolic disorders due to its antiplatelet activity [9–11].
Andrographolide has been used clinically for many years, and its cardioprotective properties are known. However, its effects on sodium (INa), calcium (ICaL), and potassium channels (IK1, IKr, Ito, IKur), and action potentials (APs) in cardiomyocytes have not been reported. This study explored the effects of andrographolide on the aforementioned ion channels and action potentials (APs) to determine its antiarrhythmic mechanism of action.
Effects of andrographolide on APs in rabbit left ventricular and left atrial myocytes
In this study, left ventricular myocytes (LVMs) and left atrial myocytes (LAMs) were isolated at the same time and were tested alternately, so comparisons between LVM and LAM electrical activity parameters were reasonable. LVMs (Figure 1A, left) were larger and wider in size than LAMs (right), and had more intensive transverse striations.
Figure 1: Effects of andrographolide (Andro) on APs, DADs, and DAD-induced TAs. Typical photomicrographs of a single LVM (left) or LAM (right) cell under 40× light microscope (A). Effects of andrographolide (5 or 10 μM) on APs recorded from rabbit LVMs (left) and LAMs (right) (B). Effect of andrographolide (5 or 10 μM) on APs stimulated at 0.5, 1, or 2 Hz (C). APs from 30 consecutive sweeps were averaged. The data of APD90 recorded at different stimulation frequencies are shown; andrographolide shortened APD90 and attenuated its RD in a concentration-dependent manner in LVMs (D). Data are shown as means±SD (n=9, #p<0.01 vs control, $p<0.01 vs 5 μM andrographolide). Andrographolide abolished ISO (1 μM) and high calcium ([Ca2+]o=3.6 mM)-induced DADs and TAs in LVMs (E). Arrows indicate depolarizing pulse.
APs were elicited by depolarizing pulses delivered in a width of 4 ms, 1.5-fold above the threshold at a rate of 1 Hz using the current-clamp technique. Figure 1B shows typical LVM (left) and LAM (right) morphology, and the effect of andrographolide on APs in these cells. Andrographolide shortened action potential duration at 50% repolarization (APD50) and 90% repolarization (APD90), and decreased maximum upstroke velocity (Vmax) in a concentration-dependent manner without changing resting membrane potential (RMP) or action potential amplitude (APA) in LVMs or LAMs. The effects of andrographolide on AP parameters were the same for LVMs and LAMs (Table 1).
Table 1: Effects of andrographolide on LVM and LAM AP parameters
-88 ± 2
-77 ± 4
-88 ± 2
-77 ± 5+
-88 ± 2
-77 ± 6+
129 ± 4
129 ± 11
129 ± 5
128 ± 11+
128 ± 4
126 ± 11+
172 ± 7
91 ± 4
147 ± 8##
77 ± 6##+
131 ± 6##$$
66 ± 4##$$+
195 ± 8
137 ± 8
164 ± 7##
119 ± 6#+
142 ± 3##$$
111 ± 6##$*
175 ± 7
249 ± 10
156 ± 8# #
226 ± 5##+
143 ± 7##
213 ± 7##$+
Data are presented as means±SD (ventricle, n=15; atrium, n=8).
##p<0.01 vs control, #p<0.05 vs control, $$p<0.01 vs 5 μM andrographolide, $p<0.05 vs 5 μM andrographolide, +p>0.05 vs ventricle, *p<0.05 vs ventricle.
RMP: resting membrane potential (mV); APA: action potential amplitude (mV); APD50: action potential duration at 50% repolarization (ms); APD90: action potential duration at 90% repolarization (ms); Vmax: maximum upstroke velocity (mV/ms).
Effects of andrographolide on rate-dependent repolarization of APs in LVMs
APs were recorded using depolarizing pulses delivered in a width of 4 ms, 1.5-fold above the threshold at a rate of 1 Hz using the current-clamp technique. APs were recorded at stimulation frequencies of 0.5, 1, and 2 Hz with or without andrographolide after the AP stabilized at 1 Hz. Andrographolide shortened APD90 in a concentration-dependent manner and attenuated rate-dependence (RD) of APD (Figure 1C–1D).
Effects of andrographolide on isoproterenol- and high calcium-induced delayed afterdepolarizations and triggered activities
APs were elicited by string stimulation containing 10 pulses at a basic cycle length (BCL) of 300 ms and string stimulation frequency of 0.125 Hz. APs were recorded after stabilization. Isoproterenol (ISO, 1 μM) was added to the external bath solution and the calcium concentration ([Ca2+]o) was increased to 3.6 mM at the same time. Under control circumstances, there were no delayed afterdepolarizations (DADs) or triggered activities (TAs). In contrast, ISO (1 μM) and high calcium ([Ca2+]o=3.6 mM) induced DADs and TAs in 7/7 LVMs following 10 consecutive pulses at a BCL of 300 ms (Figure 1E). The addition of 20 μM andrographolide abolished TAs and markedly reduced or abolished DADs.
Effects of andrographolide on sodium current (INa) in LVMs and LAMs
INa was recorded using 300 ms depolarizing voltage steps between -70 mV and +40 mV in 5 mV increments from a holding potential of -90 mV at a rate of 0.5 Hz with the cells perfused with normal bath solution and recorded the current as control group. After currents stabilized, cells were perfused with solution containing andrographolide (1, 5, 10, or 20 μM). When sealing resistance was stable, currents were recorded under different concentrations and different voltages. Results in a single cell (Figure 2A–2B) and in a group cell (Figure 2C–2D) with or without andrographolide in LVMs and LAMs showed that andrographolide decreased INa in a concentration-dependent manner without shifting the voltage at which INa amplitude was maximal.
Figure 2: Andrographolide inhibited INa in a concentration dependent manner in LVMs and LAMs. Representative whole-cell recordings of INa in LVMs (A) and LAMs (B) with or without 1, 5, 10, or 20 μM andrographolide. Current voltage relationships for INa in LVMs (C) and LAMs (D) Data are shown as means±SD (ventricle, n=10; atrium, n=8). #p<0.01 vs control, %p<0.01 vs 1 μM, $p<0.01 vs 5 μM, &p<0.01 vs 10 μM andrographolide. Representative INa recordings before (E) and after (F) andrographolide treatment using the inactivation protocol in the inset. Steady-state activation and inactivation curves for INa in LVMs (G) and LAMs (H) with or without 20 μM andrographolide. Lines represent data fit to a Boltzmann distribution function. Dose-reaction relationship between andrographolide and percent inhibition of INa (ventricle, n=10; atrium, n=10) (I)+p>0.05 vs ventricle.
Steady-state inactivation curves for sodium currents in the absence or presence of 20 μM andrographolide were evaluated from a holding potential of -90 mV. A 100 ms conditioning pre-pulse was applied from -100 mV to +40 mV in 5 mV increments followed by 100 ms depolarizing test pulses to -30 mV at a rate of 0.5 Hz to evoke INa. Figure 2E–2F show typical examples of one single cell from LVMs and LAMs, respectively. Figure 2G shows steady-state activation and inactivation curves fitted with a Boltzmann equation for INa under control conditions and after 20 μM andrographolide treatment in LVMs. For the steady-state activation of INa, with and without 20 μM andrographolide, V1/2 values were -46.28±0.31mV and -45.97±0.30 mV (n=8, p>0.05), with k=4.13±0.28 mV and 4.21±0.27 mV (n=8, p>0.05), respectively. For the steady-state inactivation of INa, with and without 20 μM andrographolide, V1/2 values were -76.63±0.38 mV and -88.52±0.84 mV (n=8, p<0.01), with k=8.60±0.45 mV and 8.25±0.53 mV (n=8, p>0.05), respectively.
Figure 2H shows the steady-state activation and inactivation curves fitted with a Boltzmann equation for INa with or without 20 μM andrographolide in LAMs. For the steady-state activation of INa, with or without 20 μM andrographolide, V1/2 values were -47.81±0.33 mV and -48.03±0.21 mV (n=8, p>0.05), with k=4.93±0.31 mV and 4.83±0.19 mV (n=8, p>0.05), respectively. For the steady-state inactivation of INa, with or without 20 μM andrographolide, V1/2 values were -79.58±0.39 mV and -88.64±0.04 mV (n=8, p<0.01), with k=9.97±0.45 mV and 9.17±0.65 mV (n=8, p>0.05), respectively. While andrographolide did not affect activation, but the voltage dependence of INa inactivation curve was shifted toward negative membrane potential, and andrographolide accelerated the inactivation process without changing its slope factor (Figure 2G–2H). Andrographolide inhibited INa in LVMs and LAMs with an IC50 of 10.41±3.18 μM and 8.28±1.26 μM, respectively (Figure 2I). The effects of andrographolide on INa were similar between LVMs and LAMs (ventricle, n=10; atrium, n=10; p>0.05 vs ventricle).
Effects of andrographolide on L-type calcium current (ICaL) in LVMs and LAMs
ICaL was recorded using a 300 ms depolarizing pulse from -40 mV to +50 mV in 5 mV increments at a rate of 0.5 Hz with a holding potential of -40 mV. One of the difficulties of studying ICaL is the run-down phenomenon in which the membrane ruptures. Figure 3A shows ICaL current density changes over time after membrane rupture without addition of any drug in LVMs. ICaL tends to stabilize at 7–25 min after membrane rupture. To show that andrographolide inhibition of ICaL was independent of the run-down phenomenon, the drug was added after ICaL peak amplitude stabilized (about 7 min after membrane rupture). The experiment was accomplished within 25 min after membrane rupture to avoid interference by the run-down phenomena.
Figure 3: Andrographolide inhibition of ICaL is reversible. ICaL time course after membrane rupture in LVMs (A). Histograms of ICaL current densities for control, 10 μM andrographolide, and washout (n=8) (B). #p<0.01 vs control, &p<0.01 vs 10 μM andrographolide). Data are shown as means±SD. Effects of andrographolide on ICaL are reversible, and nifedipine (10 μM) blocked ICaL completely in LVMs (C).
Figure 3C shows typical ICaL current traces from a single LVM cell under control conditions or with 10 μM andrographolide, washout, and 10 μM nifedipine. 10 μM andrographolide inhibited ICaL, and ICaL amplitude recovered progressively after withdrawal of andrographolide (washout). Then, to identify ICaL, current was recorded after addition of 10 μM nifedipine. ICaL was almost completely blocked by 10 μM nifedipine, indicating that the current recorded with the above pulse stimulation was ICaL. These results demonstrated that andrographolide inhibition of ICaL is significant and reversible (Figure 3B–3C).
Figure 4A–4B shows typical ICaL current traces from single LVM or LAM cells before (control) and after andrographolide treatment. ICaL current amplitude tended to stabilize within 1 min after andrographolide addition. Results in a typical single LVM or LAM cell (Figure 4A–4B) and in a group cell (Figure 4C–4D) with or without andrographolide showed that andrographolide inhibited ICaL in a concentration-dependent manner. Figure 4C–4D shows the ICaL I–V relationship after andrographolide application, which indicated that andrographolide inhibited ICaL without shifting the voltage at which ICaL amplitude was maximal.
Figure 4: Andrographolide inhibited ICaL in a concentration-dependent manner in LVMs and LAMs. Representative whole-cell recordings of ICaL in LVMs (A) and LAMs (B) with or without 1, 5, 10, or 20 μM andrographolide. Current voltage relationships for ICaL in LVMs (C) and LAMs (D) Data are shown as means±SD (ventricle, n=14; atrium, n=15). #p<0.01 vs control, % p<0.01 vs 1 μM, $ p<0.01 vs 5 μM, &p<0.01 vs 10 μM andrographolide. Representative ICaL recordings before (E) and after (F) andrographolide treatment using the inactivation protocol in the inset.Steady-state activation and inactivation curves for ICaL in LVMs (G) and LAMs (H) with or without 20 μM andrographolide. Lines represent the data fit to a Boltzmann distribution function. Dose-reaction relationship between andrographolide and percent inhibition of ICaL (ventricle, n=8; atrium, n=10) (I) +p>0.05 vs ventricle.
The steady-state ICaL inactivation curves with or without 20 μM andrographolide were evaluated from a holding potential of -40 mV. A 2000 ms conditioning pre-pulse was applied from -50 mV to 0 mV in 5 mV increments followed by 300 ms depolarizing test pulses to 0 mV at a rate of 0.5 Hz to evoke ICaL. Figure 4E–4F show typical example for one single cell of LVMs and LAMs, respectively. Figure 4G shows the steady-state activation and inactivation curves fitted with a Boltzmann equation for ICaL under control conditions and after 20 μM andrographolide application in LVMs. For the steady-state activation of ICaL, with or without 20 μM andrographolide, V1/2 values were -9.26±0.44 mV and -8.53±0.53 mV (n=14, p>0.05), with k=6.69±0.41 mV and 6.51±0.49 mV (n=14, p>0.05), respectively. For the steady-state inactivation of ICaL, with or without 20 μM andrographolide, V1/2 values were -28.44±0.23 mV and -32.87±0.35 mV (n=7, p<0.01), with k=4.55±0.21 mV and 6.09±0.31 mV (n=7, p<0.01), respectively. Figure 4H shows the steady-state activation and inactivation curves fitted with a Boltzmann equation for ICaL with or without 20 μM andrographolide in LAMs. For the steady-state activation of ICaL, with or without 20 μM andrographolide, V1/2 values were -10.99±0.31 mV and -10.66±0.33 mV (n=13, p>0.05), with k=8.32±0.33 mV and 8.89±0.37 mV (n=13, p>0.05), respectively. For the steady-state inactivation of ICaL, with or without 20 μM andrographolide, V1/2 values were -30.54±0.29 mV and -34.68±0.54 mV (n=8, p<0.01), with k=4.93±0.27 mV and 6.02±0.45 mV (n=8, p<0.01), respectively. These results suggest that andrographolide did not affect ICaL activation, but shifted the voltage dependence of ICaL inactivation curve toward negative membrane potential. Andrographolide also accelerated the inactivation process and increased its slope factor (Figure 4G–4H). Andrographolide inhibited ICaL in LVMs and LAMs with an IC50 of 11.91±1.55 μM and 10.08±1.15 μM, respectively (Figure 4I). Andrographolide had similar effects on ICaL between LVMs and LAMs (ventricle, n=8; atrium, n=10. p>0.05 vs ventricle).
Effect of andrographolide on inward rectifying potassium current (Ik1) in LVMs
IK1 was elicited by 400 ms depolarization voltage from -120 mV to +50 mV in 5 mV increments at a rate of 1 Hz with a holding potential of -40 mV. Figure 5A shows typical IK1 current traces from a single cell before and after 40 μM andrographolide treatment. Neither 20 μM nor 40 μM andrographolide affected IK1 (Figure 5C).
Figure 5: Effects of andrographolide on IK1, IKr, Ito, and IKur. IK1 (A) and its I-V relationship (C) in LVMs beforeand after andrographolide treatment. Data are shown as means±SD (n=14). Typical IKr current traces from a single LVM cell (B) and its I-V relationship (D) before and after andrographolide treatment (n=15). Representative Ito current recording (E) and its I-V relationship (F) in LAMs before and after andrographolide treatment (n=15). IKur I-V relationship in LAMs before and after application of andrographolide (n=12) (G). *p>0.05 vs control, @p>0.05 vs 10 μM andrographolide, !p>0.05 vs 20 μM andrographolide.
Effect of andrographolide on rapid delayed rectifier potassium current (IKr) in LVMs
IKr was elicited by 3000 ms depolarization voltage from -40 mV to +50 mV in 10 mV increments followed by a 5000 ms repolarization pulse to -40 mV at a rate of 0.1 Hz with a holding potential of -40 mV. Figure 5B shows typical single cell IKr current traces before and after 40 μM andrographolide application. Neither 10 μM nor 40 μM andrographolide affected IKr (Figure 5D).
Effect of andrographolide on transient outward potassium current (Ito) in LAMs
Ito was recorded using a 400 ms depolarization voltage from -40 mV to +50 mV in 10 mV increments at a rate of 0.1 Hz with a holding potential of -80 mV. INa was eliminated by 100 ms, with -40 mV depolarizing pre-pluses. Figure 5E shows typical Ito current traces from a single cell before and after 40 μM andrographolide application. Neither 20 μM nor 40 μM andrographolide affected Ito (Figure 5F).
Effect of andrographolide on ultra-rapid delayed rectifier potassium current (IKur) in LAMs
IKur was recorded with an 80 ms pre-pulse to +30 mV to inactivate Ito, then repolarized to -50 mV, lasting 50 ms, followed by a 150 ms test pulse to +60 mV from -40 mV in 10 mV increments, at a rate of 0.5 Hz with a holding potential of -50 mV. Neither 20 μM nor 40 μM andrographolide affected IKur (Figure 5G).
Effect of andrographolide on aconitine-induced ventricular arrhythmias in rabbits
Ventricular premature contraction (VPC), ventricular tachycardia (VT), and ventricular fibrillation (VF) appeared in all 10 NS group rabbits, and in 10, 7, and 1 of 10 Andro group rabbits, respectively. Andrographolide treatment prior to aconitine increased the time threshold (Figure 6A) and aconitine cumulative dosage (Figure 6B) required to induce VPC, VT, and VF compared with the NS group. Andrographolide treatment also reduced rabbit mortality (Figure 6C) and aconitine-induced ventricular arrhythmia incidence (Figure 6D–6E).
Figure 6: Effects of andrographolide on aconitine-induced arrhythmias. Histogram of the aconitine-induced arrhythmia time threshold (NS: n=10; Andro: VPC, n=10; VT, n=7) (A). Histogram of the aconitine threshold (NS: n=10; Andro: VPC, n=10; VT, n=7) (B). VPC and VT appeared in all 10 NS group rabbits, and in 10 and 7 Andro group rabbits, respectively. Rabbit mortality before and after andrographolide treatment (NS: n=10, Andro: n=10) (C). Incidence of aconitine-induced multiple ventricular arrhythmias in the two groups (D). VPC was triggered successfully in all animals, but VT and VF incidences were reduced in the Andro group. Time-dosage threshold curve of various types of ventricular arrhythmias (E). VPC, VT and VF were observed in all 10 NS group rabbits, and in 10, 7, and 1 of 10 Andro group rabbits, respectively. Typical ECG tracings showing various types of ventricular arrhythmias before (Fa) and after aconitine treatment (2 μg/kg/min) (Fb–d) VPC, VT, and VF began to appear at 17, 23, and 47 min (F). Typical ECG tracings before (Ga) and after andrographolide (10 mg/kg) and aconitine (2 μg/kg/min) treatment (Gb–d). The times of the four ECG tracings in (G) were consistent with those in (F). After andrographolide treatment, VPC appeared at 47 min, and arrhythmia did not appear at either 17 or 23 min. *p<0.01 vs NS. NS: normal saline; VPC: ventricular premature contraction; VT: ventricular tachycardia; VF: ventricular fibrillation.
This study found that andrographolide inhibited INa and ICaL in LVMs and LAMs in a concentration-dependent manner. Andrographolide (5 and 10 μM) decreased APD50, APD90, and Vmax without affecting RMP and APA in these cells. Treatment also shortened APD and attenuated RD of APD in LVMs in a concentration-dependent manner. We found that 20 μM andrographolide attenuated TAs and DADs induced by ISO (1 μM) and high calcium (3.6 mM) in LVMs. Finally, andrographolide had no influence on IK1 and IKr in LVMs, or Ito and IKur in LAMs. Our results suggest that andrographolide had cardioprotective effects in rabbits with aconitine-induced arrhythmias.
Andrographolide shifted the INa inactivation curve toward negative membrane potential and accelerated the inactivation process without changing its slope factor. Decreased INa amplitude and accelerated INa inactivation indicated that the number of Na+ flowing into the cell was reduced. Since the transient sodium current initiates the action potential , increasing the quantity of current passed through the membrane would enhance cell excitability. Thus, andrographolide decreased cell excitability, which suggests its potential use in treatment of arrhythmias caused by enhanced excitability. In cardiomyocytes, intracellular Na+ concentration ([Na+]i) is an important Ca2+ homeostasis and cell contractility modulator . [Na+]i is increased under certain pathological conditions, such as myocardial ischemia . In this study, andrographolide inhibited INa. Therefore, andrographolide reversed increased [Na+]i levels under pathological conditions by inhibiting INa, which could help alleviate the Na+-dependent calcium overload in cardiomyocytes under some pathological conditions . These results indicate that andrographolide might serve as a class I antiarrhythmic, cardioprotective therapeutic.
Normal ICaL regulation is key to intracellular Ca2+ ([Ca2+]i) homeostasis. The inorganic calcium ion (Ca2+), an important messenger in living cells, is responsible for signal transduction and regulation of vital functions . Disruption of [Ca2+]i homeostasis (calcium overload) is closely related to multiple pathological conditions, including arrhythmia , myocardial ischemia/reperfusion , heart failure , digitalis intoxication , and hypercalcinemia . Andrographolide inhibited ICaL concentration-dependently, and shifted the ICaL inactivation curve toward negative membrane potential by amplifying its V1/2 and k values. When k was increased, the inactivation process accelerated. ICaL inactivation acceleration and decreased ICaL amplitude indicated that the number of Ca2+ flowing into cell was reduced. Since andrographolide decreased [Ca2+]i, it might alleviate Ca2+ overloading in cardiomyocytes. Andrographolide could inhibit increased [Ca2+]i and restore intracellular Ca2+ homeostasis, suggesting its potential use as a class IV anti-arrhythmic drug.
Andrographolide did not influence rabbit cardiomyocyte RMP, which was consistent with our finding that it had no effect on LVM IK1. Andrographolide (5 and 10 μM) had no effect on APA, but reduced Vmax. A Vmax reduction can decrease cardiomyocyte excitability and slow down the excitement conduction velocity, which is helpful for inhibiting reentrant tachycardia. Since andrographolide had no influence on IK1, IKr, Ito, or IKur, andrographolide mainly shortens APD50 and APD90 by inhibiting ICaL. In this study, andrographolide not only shortened AP duration, but also decreased the RD of APD concentration-dependently. When RD decreased, the transmural dispersion of repolarization also diminished. Therefore, andrographolide may reduce the transmural repolarization heterogeneity of APD. Enlargement of APD transmural repolarization heterogeneity leads to the occurrence of arrhythmias . Andrographolide reduced RD, indicating that it may reduce the transmural repolarization heterogeneity of APD, thus also inhibiting reentrant arrhythmias.
ISO and high calcium causes Ca2+-overload by increasing [Ca2+]i, thereby resulting in DADs and TAs [23–25]. DAD-mediated TA can increase abnormal autorhythmicity, causing the majority of sudden cardiac deaths during nonischemic heart failure [24, 25]. In this study, 20 μM andrographolide inhibited DADs and TAs evoked by ISO and high calcium. The potential mechanism may be related to andrographolide inhibition of ICaL and INa to alleviate intracellular Ca2+- and Na+-overloading.
This study also found that andrographolide has no effect on IK1, IKr, Ito, and IKur. Enhanced reverse rate-dependence (RRD) of APD caused by drugs that inhibit IKr is an undesirable response, as it reduces drug efficacy during tachycardia and may promote proarrhythmic activity after tachycardia termination [26, 27]. Andrographolide as a potential antiarrhythmia therapeutic does not induce such side effects.
Finally, in vivo results indicated that andrographolide had cardioprotective effects in rabbits with aconitine-induced arrhythmias. Aconitine binds to voltage-dependent cardiac Na+ channels [28, 29] and prolongs their open state, favoring entry of a large quantity of Na+ into cytosol. This may be accompanied by Ca2+ overload via an electrogenic Na+-Ca2+ exchange (NCX) system, and eventually induces triggered activity [30, 31]. Furthermore, aconitinine can increase ICaL by accelerating the activation process and delaying inactivation process [32, 33]. We found that andrographolide increased the time threshold and cumulative aconitine dosage required to induce VPC, VT, and VF. It also reduced incidences of aconitine-induced VT and VF, as well as mortality in rabbits. These results indicated that andrographolide had the protective effects on aconitine-induced arrhythmias. And this antiarrhythmic effect of andrographolide was related to its inhibition of INa and ICaL.
To the best of our knowledge, this is the first demonstration about the effects of andrographolide on cardiac myocyte electrophysiologyical properties, and its possible antiarrhythmic mechanisms is related to its inhibitory effects on INa and ICaL. Our results of this study indicate that andrographolide may be a potential class I and IV antiarrhythmia agent.
MATERIALS AND METHODS
Use of rabbits in this investigation conformed to the Guide for the Care and Use of Laboratory Animals published by the National Institutes of Health (NIH publication no. 85-23, revised 1996) and the Guide for the Care and Use of Laboratory Animals (Hubei Province, China), and was approved by the Institutional Animal Care and Use Committee of Wuhan University of Science and Technology.
Single cardiac ventricular and atrial myocytes were enzymatically isolated from adult New Zealand white rabbits (1.7–2 kg weight, 24–32 weeks of age, of either sex), as described preciously . Rabbits were provided by the Experimental Animal Center of Wuhan University of Science and Technology. Rabbits were heparinized (2000 U) and anesthetized with ketamine (30 mg/kg, intravenously) and xylazine (7.5 mg/kg, intramuscularly). After the corneal reflex disappeared, rabbits were fixed on their backs to the test stands. Hearts were quickly removed after thoracotomy and put in a petri dish filled with 37°C, oxygen (95% O2 and 5% CO2) saturated, Ca2+- free Tyrode’s solution containing (mM): NaCl 135, NaH2PO4 0.33, KCl 5.4, MgCl2 1.0, HEPES 10, glucose 10 (pH 7.4, adjusted with NaOH) to stop the heartbeat. Fat and connective tissues were removed from the heart. To eliminate residual blood in the heart cavity, the aorta was cannulated and perfused retrogradely using a modified Langendorff apparatus (perfusion pressure 70 cm H2O2), then perfused for 5 more min with oxygen saturated, Ca2+-free Tyrode’s solution (at 37°C). Hearts were then digested for 30 min with the same solution containing enzyme (collagenase type I, 1 g/L) and bovine serum albumin (BSA, 1 g/L) at 37°C. The enzyme-containing solution was pumped at a constant rate using a peristaltic pump, and gas (95% O2 and 5% CO2) was allowed to pass through this solution. The perfusate was then switched to preheated and oxygen saturated Kraftbrühe (KB) solution (mM): KOH 70, KCl 40, KH2PO4 20, glutamic acid 50, taurine 20, EGTA 0.5, glucose 10, HEPES 10, MgSO4 3 (pH 7.4, adjusted with KOH) for 5 min to replace the Ca2+-free Tyrode’s solution. All solutions were bubbled with 95% O2 and 5% CO2 and maintained at 37°C. The left ventricle and left atrium were then cut into small chucks separately and gently agitated in KB solution (BSA, 1 g/L). Cells were filtered using nylon mesh and stored in KB solution (BSA, 1 g/L) until use.
Aconitine-induced arrhythmias in rabbits
Adult New Zealand white rabbits were randomly divided into two groups (n=10, each): i) Normal saline (NS) group; ii) andrographolide (Andro) group. Rabbits were then anesthetized and fixed on their backs to test stands. Polyethylene tubing was inserted into the ear marginal vein to administer aconitine, NS, and andrographolide. Standard limb lead II electrocardiogram (ECG) was measured using the BL-420F data acquisition and analysis system (Chengdu TaiMeng, Sichuan, China) following subcutaneous penetration of electrodes into four limbs. After 10 min of stabilization, NS (10 ml) was injected into NS group rabbits in 5 min through the ear marginal vein. Five min later, aconitine (2 μg/kg/min, flow rate: 80 μl/min) was injected using an infusion pump to induce arrhythmias. Andro group rabbits were treated with 10 ml andrographolide (10 mg/kg) in 5 min prior to aconitine (2 μg/kg/min, flow rate: 80 μl/min). ECG recordings were conducted in both groups for 120 min following aconitine administration. The cumulative dosage of aconitine required to induce VPC, VT and VF was calculated. VPC, VT, and VF time thresholds were recorded.
Drugs and solutions
Collagenase type I and CsCl were purchased from Gibco (Invitrogen Co., Paisley, UK). Bovine serum albumin (BSA) and HEPES were obtained from Roche (Basel, Switzerland). L-glutamic acid and taurine were purchased from Wuhan Zhongnan Chemical Reagent Co. (Wuhan, China). E-4031 and chromanol 293B were obtained from Tocris Bioscience (Minneapolis, MN, USA). All other drugs and reagents were purchased from Sigma Aldrich (Saint Louis, MO, USA). Andrographolide was dissolved in methyl alcohol, chromanol 293B in DMSO, and nifedipine in ethyl alcohol. All drugs were dissolved and diluted into the external recording solution immediately before use. Final methyl alcohol, DMSO, and ethyl alcohol concentrations in the test solutions were ≤0.1% to assure no effects on recorded currents. Stock solution of other drugs were prepared in dH2O. Drug concentrations refer to that in the external recording solution.
The AP recording bath solution contained (mM): NaCl 140, KCl 4.0, CaCl2 1.8, MgCl2 1.0, HEPES 5.0, Glucose 10.0 (pH 7.4, adjusted with NaOH) and the pipette solution contained (mM): K-aspartate 110, KCl 30, HEPES 10, EGTA 0.1, MgATP 5, Creatine phosphate 5, CAMP 0.05 (pH 7.2, adjusted with KOH).
The INa recording bath solution contained (mM): NaCl 30, CaCl2 1.0, CsCl 105, MgCl2 1.0, HEPES 5.0, Glucose 5 (pH 7.4, adjusted with CsOH) and the intracellular pipette solution contained (mM): CsCl 120, Na2ATP 5, MgCl2 5, CaCl2 1.0, TEA-Cl 10, EGTA 10, HEPES 10 (pH 7.3, adjusted with CsOH). Nifedipine (0.01 mM) was added to the bath solution to block L-type Ca2+ channels.
The ICaL recording bath solution contained (mM): NaCl 135, CsCl 5.4, CaCl2 1.8, MgCl2 1.0, BaCl2 0.3, NaH2PO4 0.33, Glucose 10, EGTA 10 (pH 7.4, adjusted with NaOH), and the pipette solution contained (mM): CsCl 120, Na2ATP 5, MgCl2 5, CaCl2 1.0, TEA-Cl 10, EGTA 10, HEPES 10 (pH 7.3, adjusted with CsOH).
Extracellular solution for IK1 recordings contained (mM): NaCl 137, KCl 5.4, CaCl2 1.8, MgCl2 1.0, NaH2PO4 0.33, HEPES 10, Glucose 10, CdCl2 0.3 (to block L-type Ca2+ channels) (pH 7.4, adjusted with NaOH). Intracellular solution for IK1 recordings contained (mM): KCl 140, MgCl2 1.0, K2ATP 5, EGTA 10, HEPES 5.0 (pH 7.3, adjusted with KOH).
The Ito and IKur recording bath solution contained (mM): NaCl 140, KCl 5.4, MgCl2 1.0, CaCl2 1.8, NaH2PO4 0.33, HEPES 5, Glucose 10 (pH 7.4, adjusted with NaOH) and the intracellular pipette solution contained (mM): KCl 20, K-aspartate 110, MgCl2 1.0, HEPES 10, EGTA 5, GTP 0.1, Na2-phosphocreatine 5, Mg2ATP 5 (pH 7.2, adjusted with KOH). For recording Ito or IKur, 200 μM BaCl2 and 200 μM CdCl2 were added to the bath solution to block IK1 and ICaL, respectively. Atropine (1.0 μM) was used to block IK,Ach. To inhibit sodium current, an inactivating pre-pulse (-40 mV, lasting 100 ms) was used when recording Ito. While recording IKur, sodium current was inhibited by a holding potential of 50 mV and equimolar N-methyl-D-glucamine replacement of Na+ in the bath solution.
For recording IKr, the external solution contained (mM): NaCl 135, KCl 5.4, CaCl2 1.0, CdCl2 0.2, NaH2PO4 0.33, MgCl2 1.0, HEPES 5, Glucose 5 (pH 7.4, adjusted with NaOH). The intracellular pipette solution contained (mM): KCl 140, MgCl2 1.0, HEPES 5, EGTA 10, Na2ATP 2 (pH 7.25, adjusted with KOH).
Transmembrane action potentials and ion currents were recorded from isolated myocytes using a patch clamp amplifier (EPC-10, Heka Electronic, Lambrecht, Pfalz, Germany) with a current or voltage clamp technique, respectively. All experiments were performed at 37±0.5°C and bath solutions were bubbled with 95% O2 and 5% CO2. Before patch clamp recording, myocytes were transferred into a recording chamber mounted on an inverted microscope stage (Nikon TE2000-S) and allowed to adhere to the glass bottom of the chamber for 5 min. A motorized micromanipulator (MP285, Sutter, USA) propelled the recording electrode to the chosen cells. Membranes were then sealed and ruptured with negative pressure. Sealing resistance was maintained >1GΩ. A 80% compensation of series resistance was achieved without ringing. Capacitance and series resistances were adjusted to minimize the contribution of the capacitive transients. Patch electrodes were pulled with a two-stage patch pipette puller (PP-830, Narishige Group, Tokyo, Japan) and then fire-polished. Patch electrodes had a resistance of 1.8–2.5 MΩ when filled with pipette solution. Current signals were conducted by the Ag/AgCl electrode and amplified by an EPC-10 amplifier, then filtered at 1.5 kHz, digitized at 10 kHz, and stored on a computer hard disk for analysis.
Applicate FitMaster (v2x32; HEKA) was used for data analysis and SPSS 18.0 for statistical analysis. Figures were plotted using Origin software (V7.0, OriginLab Co., MA, USA). Summary data were presented as means±SD. Current density was obtained by dividing current amplitude by cell capacitance. Data from steady-state INa activation and inactivation were fitted to the Boltzmann equation: Y=1/[1+exp(Vm -V1/2)/k], where Vm is the membrane potential, V1/2 the half-activation or half-inactivation potential, and k the slope factor. For steady-state activation curves, Y represents relative conductance. Chord conductance was calculated using the ratio of the current to electromotive force for potential in individual current-voltage relationships. Conductances were normalized to their individual maximal conductance. For steady-state inactivation curves, Y represents relative current (INa/INamax; ICaL/ICaLmax). Differences between groups were determined using one-way analysis of variance (ANOVA) followed by the Tukey multiple comparison test or Student’s paired t-test. P<0.05 was considered statistically significant.
CONFLICTS OF INTEREST
The authors declare no conflicts of interest.
This work was supported by the National Natural Science Foundation of China (No 81670302).
1. Ren J, Liu Z, Wang Q, Giles J, Greenberg J, Sheibani N, Kent KC, Liu B. Andrographolide ameliorates abdominal aortic aneurysm progression by inhibiting inflammatory cell infiltration through downregulation of cytokine and integrin expression. J Pharmacol Exp Ther. 2016; 356:137-147.
2. Kishore V, Yarla NS, Bishayee A, Putta S, Malla R, Neelapu NR, Challa S, Das S, Shiralgi Y, Hegde G, Dhananjaya BL. Multi-targeting andrographolide and its natural analogs as potential therapeutic agents. Curr Top Med Chem. 2017; 17:845-857.
3. Wong SY, Tan MG, Wong PT, Herr DR, Lai MK. Andrographolide induces Nrf2 and heme oxygenase 1 in astrocytes by activating p38 MAPK and ERK. J Neuroinflammation. 2016; 13:251.
4. Xu F, Wu H, Zhang K, Lv P, Zheng L, Zhao J. Proneurogenic effects of andrographolide on RSC96 Schwann cells in vitro. Mol Med Rep. 2016; 14:3573-3580.
5. Awang K, Abdullah NH, Hadi AH, Fong YS. Cardiovascular activity of labdane diterpenes from Andrographis paniculata in isolated rat hearts. J Biomed Biotechnol. 2012; 2012:876458.
6. Woo AY, Waye MM, Tsui SK, Yeung ST, Cheng CH. Andrographolide up-regulates cellular-reduced glutathione level and protects cardiomyocytes against hypoxia/reoxygenation injury. J Pharmacol Exp Ther. 2008; 325:226-235.
7. Trivedi NP, Rawal UM. Hepatoprotective and antioxidant property of Andrographis paniculata (Nees) in BHC induced liver damage in mice. Indian J Exp Biol. 2001; 39:41-46.
8. Zhang J, Zhu D, Wang Y, Ju Y. Andrographolide attenuates LPS-induced cardiac malfunctions through inhibition of IkappaB phosphorylation and apoptosis in mice. Cell Physiol Biochem. 2015; 37:1619-1628.
9. Lien LM, Su CC, Hsu WH, Lu WJ, Chung CL, Yen TL, Chiu HC, Sheu JR, Lin KH. Mechanisms of andrographolide-induced platelet apoptosis in human platelets: regulatory roles of the extrinsic apoptotic pathway. Phytother Res. 2013; 27:1671-1677.
10. Lu WJ, Lin KH, Hsu MJ, Chou DS, Hsiao G, Sheu JR. Suppression of NF-kappaB signaling by andrographolide with a novel mechanism in human platelets: regulatory roles of the p38 MAPK-hydroxyl radical-ERK2 cascade. Biochem Pharmacol. 2012; 84:914-924.
11. Wang YJ, Wang JT, Fan QX, Geng JG. Andrographolide inhibits NF-kappaBeta activation and attenuates neointimal hyperplasia in arterial restenosis. Cell Res. 2007; 17:933-941.
12. Kuksis M, Ferguson AV. Actions of a hydrogen sulfide donor (NaHS) on transient sodium, persistent sodium, and voltage-gated calcium currents in neurons of the subfornical organ. J Neurophysiol. 2015; 114:1641-1651.
13. Bay J, Kohlhaas M, Maack C. Intracellular Na(+) and cardiac metabolism. J Mol Cell Cardiol. 2013; 61:20-27.
14. Williams IA, Xiao XH, Ju YK, Allen DG. The rise of [Na(+)] (i) during ischemia and reperfusion in the rat heart-underlying mechanisms. Pflugers Arch. 2007; 454:903-912.
15. Zhang S, Ma JH, Zhang PH, Luo AT, Ren ZQ, Kong LH. Sophocarpine attenuates the Na(+)-dependent Ca2(+) overload induced by Anemonia sulcata toxin-increased late sodium current in rabbit ventricular myocytes. J Cardiovasc Pharmacol. 2012; 60:357-366.
16. Berridge MJ. Elementary and global aspects of calcium signalling. J Physiol. 1997; 499:291-306.
17. Fan X, Ma J, Wan W, Zhang P, Wang C, Wu L. Increased intracellular calcium concentration causes electrical turbulence in guinea pig ventricular myocytes. Sci China Life Sci. 2011; 54:240-247.
18. de Diego C, Pai RK, Chen F, Xie LH, De Leeuw J, Weiss JN, Valderrabano M. Electrophysiological consequences of acute regional ischemia/reperfusion in neonatal rat ventricular myocyte monolayers. Circulation. 2008; 118:2330-2337.
19. Casini S, Verkerk AO, van Borren MM, van Ginneken AC, Veldkamp MW, de Bakker JM, Tan HL. Intracellular calcium modulation of voltage-gated sodium channels in ventricular myocytes. Cardiovasc Res. 2009; 81:72-81.
20. Rocchetti M, Besana A, Mostacciuolo G, Ferrari P, Micheletti R, Zaza A. Diverse toxicity associated with cardiac Na+/K+ pump inhibition: evaluation of electrophysiological mechanisms. J Pharmacol Exp Ther. 2003; 305:765-771.
21. Shutt RH, Ferrier GR, Howlett SE. Increases in diastolic [Ca2+] can contribute to positive inotropy in guinea pig ventricular myocytes in the absence of changes in amplitudes of Ca2+ transients. Am J Physiol Heart Circ Physiol. 2006; 291:H1623-1634.
22. Walton RD, Martinez ME, Bishop MJ, Hocini M, Haissaguerre M, Plank G, Bernus O, Vigmond EJ. Influence of the Purkinje-muscle junction on transmural repolarization heterogeneity. Cardiovasc Res. 2014; 103:629-640.
23. Sicouri S, Belardinelli L, Antzelevitch C. Antiarrhythmic effects of the highly selective late sodium channel current blocker GS-458967. Heart Rhythm. 2013; 10:1036-1043.
24. Zhao YT, Valdivia CR, Gurrola GB, Hernandez JJ, Valdivia HH. Arrhythmogenic mechanisms in ryanodine receptor channelopathies. Sci China Life Sci. 2015; 58:54-58.
25. Asakura K, Cha CY, Yamaoka H, Horikawa Y, Memida H, Powell T, Amano A, Noma A. EAD and DAD mechanisms analyzed by developing a new human ventricular cell model. Prog Biophys Mol Biol. 2014; 116:11-24.
26. Dorian P, Newman D. Rate dependence of the effect of antiarrhythmic drugs delaying cardiac repolarization: an overview. Europace. 2000; 2:277-285.
27. Grom A, Faber TS, Brunner M, Bode C, Zehender M. Delayed adaptation of ventricular repolarization after sudden changes in heart rate due to conversion of atrial fibrillation. A potential risk factor for proarrhythmia? Europace. 2005; 7:113-121.
28. Catterall WA. Structure and function of voltage-sensitive ion channels. Science. 1988; 242:50-61.
29. Catterall WA. From ionic currents to molecular mechanisms: the structure and function of voltage-gated sodium channels. Neuron. 2000; 26:13-25.
30. Sawanobori T, Hirano Y, Hiraoka M. Aconitine-induced delayed afterdepolarization in frog atrium and guinea pig papillary muscles in the presence of low concentrations of Ca2+. Jpn J Physiol. 1987; 37:59-79.
31. Watano T, Harada Y, Harada K, Nishimura N. Effect of Na+/Ca2+ exchange inhibitor, KB-R7943 on ouabain-induced arrhythmias in guinea-pigs. Br J Pharmacol. 1999; 127:1846-1850.
32. Zhao Z, Yin Y, Wu H, Jiang M, Lou J, Bai G, Luo G. Arctigenin, a potential anti-arrhythmic agent, inhibits aconitine-induced arrhythmia by regulating multi-ion channels. Cell Physiol Biochem. 2013; 32:1342-1353.
33. Zhou YH, Piao XM, Liu X, Liang HH, Wang LM, Xiong XH, Wang L, Lu YJ, Shan HL. Arrhythmogenesis toxicity of aconitine is related to intracellular ca(2+) signals. Int J Med Sci. 2013; 10:1242-1249.
34. Ren Z, Ma J, Zhang P, Luo A, Zhang S, Kong L, Qian C. The effect of ligustrazine on L-type calcium current, calcium transient and contractility in rabbit ventricular myocytes. J Ethnopharmacol. 2012; 144:555-561.
All site content, except where otherwise noted, is licensed under a Creative Commons Attribution 3.0 License.