Oxidative Medicine and Cellular Longevity

Oxidative Medicine and Cellular Longevity / 2021 / Article
Special Issue

New Molecules and Mechanisms to Fight the Onset and Progression of Cardiovascular Diseases

View this Special Issue

Research Article | Open Access

Volume 2021 |Article ID 9912434 | https://doi.org/10.1155/2021/9912434

Judith Bernal-Ramírez, Christian Silva-Platas, Carlos Jerjes-Sánchez, Martín R. Ramos-González, Eduardo Vázquez-Garza, Héctor Chapoy-Villanueva, Alicia Ramírez-Rivera, Ángel Zarain-Herzberg, Noemi García, Gerardo García-Rivas, "Resveratrol Prevents Right Ventricle Dysfunction, Calcium Mishandling, and Energetic Failure via SIRT3 Stimulation in Pulmonary Arterial Hypertension", Oxidative Medicine and Cellular Longevity, vol. 2021, Article ID 9912434, 15 pages, 2021. https://doi.org/10.1155/2021/9912434

Resveratrol Prevents Right Ventricle Dysfunction, Calcium Mishandling, and Energetic Failure via SIRT3 Stimulation in Pulmonary Arterial Hypertension

Academic Editor: Gaetano Santulli
Received05 Mar 2021
Revised20 May 2021
Accepted25 May 2021
Published21 Jun 2021

Abstract

Pulmonary arterial hypertension (PAH) is characterized by pulmonary vessel remodeling; however, its severity and impact on survival depend on right ventricular (RV) failure. Resveratrol (RES), a polyphenol found in red wine, exhibits cardioprotective effects on RV dysfunction in PAH. However, most literature has focused on RES protective effect on lung vasculature; recent finding indicates that RES has a cardioprotective effect independent of pulmonary arterial pressure on RV dysfunction, although the underlying mechanism in RV has not been determined. Therefore, this study is aimed at evaluating sirtuin-3 (SIRT3) modulation by RES in RV using a monocrotaline- (MC-) induced PAH rat model. Myocyte function was evaluated by confocal microscopy as cell contractility, calcium signaling, and mitochondrial membrane potential (); cell energetics was assessed by high-resolution respirometry, and western blot and immunoprecipitation evaluated posttranslational modifications. PAH significantly affects mitochondrial function in RV; PAH is prone to mitochondrial permeability transition pore (mPTP) opening, thus decreasing the mitochondrial membrane potential. The compromised cellular energetics affects cardiomyocyte function by decreasing sarco-endoplasmic reticulum Ca2+-ATPase (SERCA) activity and delaying myofilament unbinding, disrupting cell relaxation. RES partially protects mitochondrial integrity by deacetylating cyclophilin-D, a critical component of the mPTP, increasing SIRT3 expression and activity and preventing mPTP opening. The preserved energetic capability rescues cell relaxation by maintaining SERCA activity. Avoiding Ca2+ transient and cell contractility mismatch by preserving mitochondrial function describes, for the first time, impairment in excitation-contraction-energetics coupling in RV failure. These results highlight the importance of mitochondrial energetics and mPTP in PAH.

1. Introduction

Pulmonary arterial hypertension (PAH) is a complex disease resulted from the interplay of several biological and environmental processes leading to pulmonary vasculature remodeling, therefore pulmonary hypertension [1]. Consequently, the low-pressure, thin-walled, crescent-shaped RV has to overcome structural changes to accomplish its function and pump against such an increased afterload [2]. Therefore, RV hypertrophy is a necessary adaptation to preserve RV-pulmonary arterial coupling by decreasing RV wall tension and increasing RV cardiomyocyte force-generating capacity [2]. Consequently, in early stages, it emerges as an adaptative remodeling, while at end stage of the disease, it becomes a maladaptive remodeling [2]. Despite the publication of 41 randomized clinical trials in the past 25 years and the regulatory approval of multiple drugs delivered by four administration routes [3], there is no drug focused on improving RV performance and/or reducing inflammation [4]. Despite currently available therapies PAH patients remain significant morbidity and mortality [1]. A polyphenol from the stilbene family, 3,5,4-trihydroxystilbene resveratrol (RES), has drawn researchers’ attention by its cardioprotective activity in other cardiovascular diseases [5]. Although RES acts as a pleiotropic agent in several conditions, it has an intrinsic antioxidant capacity, as well as an ability to regulate membrane receptors, kinases, and other enzymes [68]. In PAH models, RES improves lung functioning through its antiproliferative [9], antioxidant [10], and anti-inflammatory properties [11]. More precisely, RES activates sirtuins, a relevant group of deacetylases that participate in the regulation of numerous cellular processes [12]. In the heart, sirtuin activation has been linked to the prevention of hypertrophy [13] and energetic dysfunction [14, 15].

Previously, we found the prevention of RV hypertrophy and cardiac fibrosis by RES in PAH, accompanied by a decrease in the RV acetylation profile [16]. However, the connection between these two mechanisms remains unclear. Progression to RV failure has been linked to mitochondrial dysfunction [17, 18], as PAH generates a disruption in the mitochondrial structure [17], decreasing its oxidative capability [19] and diminishing ATP production [17, 20]. The compromised cardiac energetics impairs RV contractility by reducing creatine kinase expression [21], a key component in transferring energy to myofilaments. Thus, protecting mitochondrial function with cyclosporine A (CsA), which blocks mPTP opening by interacting with cyclophilin D (CypD), prevents mitochondrial disruption in PAH and preserves RV function [22]. CypD hyperacetylation is an essential trigger of mPTP opening [23], and its contribution to mitochondrial dysfunction and heart failure has been established in animal models [24] and humans [15]. Notably, CypD acetylation is regulated by SIRT3 [23, 24], a sirtuin stimulated by RES [12], which is associated with the loss-of-function polymorphism found in PAH patients [25].

The search for additional therapeutic options for more effective PAH management has led to the development and approval of new drugs [26]; however, the available treatments focus on exclusively in managing pulmonary alterations [27]. Gaining a basic understanding of RV alterations through dysfunction, RV failure, and mechanisms that delay these changes may be helpful in developing new therapeutic strategies to improve PAH prognosis. Therefore, the aim of this study is to evaluate the extent of SIRT3 activation in the cardioprotection conferred by RES in the RV of a MC-induced PAH model.

2. Materials and Methods

2.1. Reagents

All reagents were purchased from Sigma-Aldrich (St. Louis, MO, USA), unless otherwise stated.

2.2. Murine Model of Pulmonary Arterial Hypertension

PAH was induced in male Sprague–Dawley rats (Bioinvert, Edo. de México, MX) weighing >300 g by a single MC (PHL8925) dose (60 mg/kg, subcutaneous) diluted in dimethylsulfoxide (DMSO, 472301), as previously reported [16]. The control group was treated with equivalent volume of DMSO. Animals were kept at 25°C with 12 h light/dark cycle. Water and food were given ad libitum. A group of MC-injected animals was treated with RES dissolved in water (20 mg/kg/day, intra gastric) during day 1 to 42 after MC injection (PAH-RES) [16]. The other groups were given equivalent volume of water (intragastric). All animals were observed for general appearance and respiratory symptomatology. A group of control animals treated with RES during 42 days (20 mg/kg/day, intragastric) was evaluated.

2.3. Histologic Preparations

As reported previously [16], after injection of sodium heparin (1000 U/kg), animals were anesthetized with 5% sevoflurane and the heart and lungs were removed to be fixed in 4% (wt/vol) paraformaldehyde in PBS at room temperature for more than 2 hours. Afterwards, tissues were embedded in paraffin and stained with hematoxylin/eosin (H&E) and Masson’s trichrome. An Imager Z1 Zeiss microscope with an AxioCam HRm was used, and images were processed with the AxioVision software. Micrograph from the whole Masson’s trichrome stained slides was taken at 2.5x; then, the image was decomposed in more than 7 fields at 5x. Fibrotic index was assessed by quantification of blue and red pixels, using ImageJ (http://imagej.nih.gov/ij/, NIH, Bethesda, MD, USA); a blue%/red% ratio was made. Two blinded analysts performed the analysis, and three different fields were analyzed. H&E micrograph from the papillary muscles was used to quantify cardiomyocyte area at 10x. An object carrier with a capacity for 7 slides was used to analyze all slides with their respective batches. Arterioles with smooth muscular medial layer proliferation were quantified in seven random fields of lung H&E micrograph, to analyze its diameter, and the occlusion vessel of 100 μm was selected. Occlusion was obtained by averaging more than seven measurements of the medial layer thickness.

2.4. Cardiomyocyte Isolation

Ventricular myocytes were isolated modifying a previous report [28]. Briefly after, animals were heparinized (1000 U/kg, intraperitoneal) and anesthetized with sevoflurane (1.5%-3%/1 L/min, inhaled). Hearts were excised and mounted on a Langendorff apparatus to be perfused with Tyrode solution (Ty) (mM: 128 NaCl, 0.4 NaH2PO4, 6 glucose, 5.4 KCl, 0.5 MgCl-6H2O, 5 creatinine, 5 taurine and 25 HEPES, pH 7.4) at 37°C for 5 min and digested by collagenase type II (0.1% in Ty) (Worthington Biochemical, Lakewood, NJ). Subsequently, RV was dissected and cells were mechanically disaggregated. Cardiomyocytes were rinsed with 0.1% albumin in Ty solution at increasing Ca2+ concentrations (0.25, 0.5, and 1 mM). All the confocal measurements were acquired using a Leica TCS SP5 confocal microscope equipped with a D-apochromatic 63X, 1.2 NA, oil objective (Leica Microsystems, Wetzlar, Germany). Only rod-shaped cells with visible striations were selected for the study. All records were analyzed using ImageJ (http://imagej.nih.gov/ij/, NIH, Bethesda, MD, USA).

2.5. Cell Shortening and Ca2+ Handling in Intact Cardiomyocytes

Cell shortening was evaluated in 0.5 Hz paced Ca2+ transient records, where the scanned line was longer than the cell length, following a previous report [29]. Briefly, a rectangular region comprising both cellular edges was selected and a threshold was set to distinguish the intracellular from the extracellular space, converting the image into binary. The cell border of the resulting binary image was compared to the border on the original record to ensure a close fit. Cell shortening parameters evaluated were time to peak shortening from fully cell rest length and time to 50% of relaxation from maximal shortening. ImageJ software (http://imagej.nih.gov/ij/, NIH, Bethesda, MD, USA) was used to process images. Intracellular Ca2+ signaling was measured as previously reported [28, 30]. Recently isolated cardiomyocytes were incubated with 10 μM Fluo-4 AM (F14201, Life Technologies, USA) (in Ty, 1 mM Ca2+) for 45 min at 25°C. Later, cells were washed with fluorophore-free solution, plated on laminin- (L2020) covered glass coverslips, and mounted in a superfusion chamber. Line scan images were recorded by the cell longitudinal axis (400 Hz, 1 μm section thickness) by confocal microscopy under 0.5 Hz field stimulation (MYP100 MyoPacer Field Stimulator; Ion-Optix, Milton, MA, USA). Fluorophore excitation was 488 nm, and emission window was 500-600 nm. β-Adrenergic stimulation was assessed after 10 min of 100 nM isoproterenol (16504) (ISO in Ty, 1 mM Ca2+) perfusion at 1 Hz stimulation. Fluorescence data is shown as , where is the average fluorescence intensity before field stimulation. To evaluate spark characteristics in freshly isolated myocytes, the longitudinal cell axis with 100 nm pixel size records was taken at 1 Hz pace. Analysis was performed using ImageJ software (http://imagej.nih.gov/ij/, NIH, Bethesda, MD, USA) with the SparkMaster plugin [31].

2.6. Mitochondrial Membrane Potential in Intact Cardiomyocytes

Freshly isolated cardiomyocyte cells were incubated with 300 nM tetramethylrhodamine ethyl ester perchlorate (TMRE) (T669, Thermo Fisher Scientific, USA) for 30 min at 25°C (in Ty, 1 mM Ca2+) [32]. After washing with a fluorophore-free and Ca2+-free solution, 2D images ( pixels, 400 Hz, 1 μm section thickness) were taken using 543 nm excitation and 555-700 nm emission window. Results were normalized to the CTRL group as a percentage. The degree of mitochondrion polarization was then expressed as TMRE intensity per cell. As a negative control, cells were perfused with 0.8 μM cyanide m-chlorophenyl hydrazone (CCCP) (C2759) during 10 min (data not shown).

2.7. Mitochondrial Isolation

Heart mitochondrial fractions were obtained according to the method described previously [33]. Briefly, the heart was isolated and placed in an ice-cold buffer (SHE), containing (mM) the following: 250 sucrose, 10 HEPES and 1 EGTA, and pH 7.3. After, only RV tissue was digested for 10 min using 0.12 mg of protease in cold SHE buffer and centrifuged at 800 x g. The homogenates were centrifuged at 10000 x g for 10 min, and then the resulting pellet was suspended in SH buffer containing (mM) the following: 250 sucrose, 10 HEPES, pH 7.3, and free EGTA. Isolated mitochondria were suspended (0.6 mg/ml) in respiration buffer containing (in mM) the following: 125 KCl, 3 KH2PO4, 10 HEPES, and pH 7.3.

2.8. Mitochondrial Function from RV in the PAH Model

For the respiratory studies, 0.1 mg/ml mitochondria in respiratory medium (140 mM K+-gluconate, 5 mM KH2PO4, 2 μg/ml rotenone, 10 mM succinate, 10 mM HEPES pH 7.2) was evaluated during the respiratory states of no-phosphorylation (state 4), phosphorylation (state 3, ADP added), and maximal respiratory activity (uncoupled with FCCP). Oxygen consumption was recorded using high-resolution respirometry (Oroboros Instrument, Innsbruck, Austria) [32].

2.9. Ca2+ Retention Capacity (CRC)

mPTP opening sensitivity was evaluated in isolated mitochondrial by CRC. Mitochondria were incubated in a medium containing 0.3 μM Calcium Green-5N (C3739, Life Technologies, Carlsbad, CA, US), 10 mM succinate plus rotenone (10 μg/ml), 200 μM ADP, and 0.25 μg Oligomycin A. After 5-minute incubation, 10 μM of Ca2+ pulses was added every 3 min and fluorescence was recorded at 488 nm excitation and 500-600 nm emission. After enough Ca2+ loading, a massive release of mitochondrial Ca2+ indicates mPTP opening. The amount of CaCl2 necessary to trigger this enormous Ca2+ release was used as an indicator of the susceptibility to mPTP opening due to Ca2+ overload [32].

2.10. Protein Extraction

50 mg heart tissue was macerated using a Polytron PT1200 E (Kinematica AG, Switzerland) with 500 μl of buffer SHE added with 1 mM phenylmethylsulfonyl fluoride (PMSF, P7626) and 1 mM dithiothreitol (DTT, D0632). Afterwards, the homogenate was centrifuged at 2000 rpm during 10 min at 4°C. Protein was quantified in the supernatant by the Lowry method using bovine serum albumin as standard.

2.11. Western Blot

Protein were resolved on SDS-PAGE gel and transferred onto a PVDF membrane, which was incubated with primary antibody. The membrane was washed three times for 10 min with PBS-0.5% Tween 20 and subsequently probed with an HPR-conjugated secondary for 2 hours at 25°C. After washing three times with PBS-0.5% Tween 20 for 10 min, the blots were developed with SuperSignal West Dura Extended Duration Substrate (TG268239, Thermo Fisher Scientific, Waltham, MA, US) and quantified by using a BioSpectrum 415 Image Acquisition System (UVP, Upland, CA, USA). Protein acetylation used 30 μg of isolated mitochondria in a 15% SDS-PAGE gel;to SIRT3 expression, 15 μg of isolated mitochondria was used in a 12% SDS-PAGE gel; electrophoresis and transfer conditions were 105 V, 25°C, 2.5 h, and 300 mA, 4°C, 2 h, respectively, to both. SERCA2, phospholamban (PLB), and D-glyceraldehyde-3-phosphate dehydrogenase (GAPDH) were quantified in the same blot. 40 μg of tissue homogenate was loaded in 12% SDS-PAGE gel. Electrophoresis and transfer conditions were 85 V, 25°C, 2 h, and 350 mA, 25°C, 1.5 h, respectively. Primary antibodies used were as follows: anti-Acetylated-Lysine (9441S, Cell Signaling, Danvers, MA, US) (1 : 1000); anti-SIRT3 (D22A3, Cell Signaling, Danvers, MA, US) (1 : 2000); anti-SERCA (sc-8094, Santa Cruz Biotechnology, MA, US) (1 : 10000); and anti-PLB (sc-21923, Santa Cruz Biotechnology, MA, US) (1 : 1000). Anti-COX4 (4D11-B3-E8, Cell Signaling, Danvers, MA, US) (1 : 2000) [25] and anti-GAPDH (sc-25778, Santa Cruz Biotechnology, MA, US) (1 : 10000) antibodies were used as a loading control.

2.12. Real-Time Polymerase Chain Reaction (PCR) Analysis

Total RNA from right ventricles was extracted using TRIzol Reagent (15596026, Invitrogen, Carlsbad, CA, USA). Sample purity was confirmed measuring a 260/280 nm absorbance ratio using a Take3 multivolume plate in a Synergy HT microplate reader (BioTek Instruments, Winooski, USA). SensiFAST cDNA Synthesis Kit (BIO-65053, Bioline, London, UK) was used to reverse-transcribe cDNA from 1 μg of total RNA. qPCR reaction was performed using the SensiFAST SYBR Lo-ROX Kit (BIO-94020, Bioline, London, UK) in a Quant-Studio 3 RT PCR System (Thermo Fisher Scientific, Waltham, TX, USA). Data was analyzed by 2−ΔΔCt method to estimate mRNA expression from each gene [15, 34]. T4 Oligo (Mexico) synthesized primers. Primer sequences are detailed in Supplementary Table 1.

2.13. Oxidative Stress Markers

Free thiol groups were evaluated in 200 μg of isolated mitochondria incubated with 5,5-dithio-bis-(2-nitrobenzoic acid) (DNTB, 300 μM) (D8130), during 10 min at 25°C in darkness. After 10 min centrifugation at 10000 rpm, the supernatant was measured at 412 nm. Protein carbonyl content was assessed in homogenized tissue following assay kit (ab126287, Abcam, UK) instructions. Membrane lipid peroxidation was analyzed by measuring the generation of thiobarbituric acid-reactive substances (TBARS) as previously reported [35]. DNA oxidation was analyzed by ELISA assay according to the kit manufacturer’s instructions (ab101245, Abcam, UK). The concentration of 8-hydroxy-20-deoxyguanosine (8-OHdG) was measured using a standard curve and expressed in nanograms per micrograms of DNA [36]. Enzyme activities were evaluated in a homogenized heart tissue. Catalase activity was measured by O2 production assessed by an electrode type Clark [36]. Briefly, 50 μg protein was added to phosphate buffer (KH2PO4 50 mM, pH 7.8), and the addition of 5 mM H2O2 (quantified at 240 nm with an extinction coefficient of ) started the reaction. Data were expressed as units per milligram of protein (U/mg). Aconitase activity was measured by monitoring cis-aconitate synthesis from citrate at 30°C on 240 nm. 150 μg protein was added to 1 ml of medium (100 mM KH2PO4, 0.01% Triton X-100, 0.6 mM MnCl2, 0.2 mM NADP, and 1 mM citrate, pH 7.2). Enzyme activity is expressed as , using cis-aconitate extinction coefficient (). Superoxide dismutase activity was measured as previously reported [36]. Briefly, 50 μg protein was added to phosphate buffer (50 mM KH2PO4, 1 mM EDTA, 10 mM xanthine, 50 μM nitro-blue tetrazolium chloride (NBT), 1 U catalase, 1.5 U Xantina oxidase, pH 7.8). Oxidation of NBT by superoxide anion was measured at 560 nm. To measure Mn-SOD, 3 mM KCN was added. One activity unit was defined as 50% oxidation of NBT. Results were expressed as units per milligram of protein (U/mg).

2.14. Immunoprecipitation

As described before [15], isolated mitochondria from right ventricles (1 mg) were solubilized in buffer containing (in mM) the following: 150 NaCl, 1 EGTA, Igepal 1%, 20 Tris-HCl, pH 7.2, and protease inhibitor cocktail (Roche). Afterwards, they were clarified of endogenous IgG and incubated with 2 μg of mouse anti-CypD (ab110324, Abcam, UK), or the isotype IgG as control, 1 hour at 4°C in a rotator. The immunoprecipitation complexes were captured by adding 50% activated slurry of Protein G Sepharose beads (GE) to the solubilized protein and incubated overnight at 4°C in a rotator. Beads were centrifuged and washed thrice. Complexes were eluted in SDS-loading buffer prior to electrophoretic separation and subsequent western blot analysis.

2.15. Statistics

Data is presented as the . Statistical analysis and graphs were performed using GraphPad Prism software (V.5.01; La Jolla, CA, USA). Data were analyzed by one-way ANOVA or two-tailed Student’s -test;to compare the groups, Dunn’s post hoc test was performed when appropriate. Statistical significance was set at .

2.16. Study Approval

All procedures performed in animals were supervised and approved by the Internal Committee for Care and Handling of Laboratory Animals of the School of Medicine of the Tecnológico de Monterrey (Protocols no. 2017-006 and 2019-019) and were performed following the Mexican National Laboratory Animal Health Guidelines (NOM 062-ZOO 1999).

3. Results

3.1. RES Preserves Right Ventricular Function with a Limited Effect on Lung Vasculature

The PAH model requires 28–42 days to develop phenotypic changes in the lungs and heart [37]. Previously, it has been shown that heart alterations caused by MC target the RV and RES treatment improve RV function with a limited protective effect on pulmonary architecture [16]. In addition, rats treated only with RES showed no differences compared to the control animals (without MC) for lung morphological parameters such avessel lumen diameter, number of muscular arteries, luminal occlusion, and RV histological characteristics (Supplemental Figure 1).

3.2. RES Prevents Contractility Alterations and Improves Ca2+ Handling

RV myocyte function was evaluated by characterizing cell contraction and Ca2+ dynamics to assess alterations in excitation-contraction coupling (ECC). Cell shortening was less efficient in the PAH group since time to peak shortening (Figure 1(b)) and half relaxation (Figure 1(c)) were 82% and 41% slower, respectively. RES treatment accelerated the time to peak shortening by 22% in PAH (Figure 1(b)) and maintained the CTRL group time to half relaxation (Figure 1(c)), indicating that RES treatment improved cell relaxation in PAH.

Since intracellular Ca2+ dynamics orchestrates cell contractility, transient parameters were characterized. Transient amplitude (Figure 1(e)) did not change between groups. However, in transient decay, the PAH group showed a 1.2-fold slower than CTRL, while RES reduced this effect by 26% (Figure 1(f)); however, no significant differences were shown in the SERCA2/PLB ratio between the PAH and PAH+RES groups (Figure 1(g)), indicating that the improved might have been due to increased SERCA activity rather than changes in its expression. Gene expression of other Ca2+ extrusion mechanisms, Na/Ca2+ exchanger (NCX) and mitochondria calcium uniplex (MCU), did not change between groups (NCX: , , PAH+; MCU: , , PAH+ mRNA/HPRT).

Ca2+ spark frequency (Figure 1(i)) and amplitude (Figure 1(j)) were measured as an indicative of RyR activity. No changes were observed between PAH and CTRL groups; thus, RyR activity was not affected. However, the PAH-RES group had a higher spark amplitude than the PAH group (PAH: , RES+PAH: , ), suggesting a higher SR Ca2+ content.

RV myocytes were challenged after isoprenaline (ISO, 100 nM) perfusion to induce the β-adrenergic response (β-AR), a highly energy-dependent state (Supplemental. Fig. 2). All groups were capable to increase Ca2+ transient amplitude and to reduce . However, cell contraction failed to comply in the PAH group, while RES-treated PAH prevented this Ca2+ transient and cell contractility mismatch.

3.3. RES Prevents Cellular Energetics Failure

Since β-AR emphasizes the disruption of excitation-contraction-energetic coupling (ECEC) in PAH, mitochondrial function was evaluated in isolated myocytes and mitochondria from the RV tissue. PAH compromises ATP production by altering mitochondrial functioning, as decreased by 47% in PAH myocytes (), while in RES-treated PAH, the control level was sustained (%) (Figure 2(b)). RV mitochondria from the PAH group also showed a 26% reduction in respiratory activity during state 3 of respiration (Figure 2(c)) with no change in basal respiratory activity in state 4 (Figure 2(d)), thus decreasing respiratory control ratio (CTRL: ; PAH: ) (Figure 2(e)). In the PAH-RES group, mitochondria maintained the respiratory control ratio () (Figure 2(e)) by preserving the phosphorylation response (CTRL:  nmol O2/min∙mg; PAH+RES:  nmol O2/min∙mg) (Figure 2(c)). Isolated mitochondria from the PAH group also showed increased mPTP, demonstrated by an 81% decrease in Ca2+ retention capacity (CRC), while RES treatment produced a 2.5-fold decrease in mitochondrial fragility in the PAH-RES group (Figure 2(f)). The enhanced permeability was a consequence of mPTP opening since the effect is inhibited by CsA, a potent inhibitor of the mPTP (: nmol Ca2+/mg, nmol Ca2+/mg, PAH+ nmol Ca2+/mg; ; : 7, 6, and 5 mitochondrial preparations, respectively).

The involvement of oxidative stress in mitochondria permeability transitioning was also evaluated. As shown in Figure 3(b), there was an increase in membrane peroxidation concomitant with 48% decrease in aconitase activity in the PAH group indicating an increased oxidant environment within the mitochondria. However, other antioxidant enzymes and oxidation in protein or DNA did not change in the PAH group (Figure 3). RES treatment maintained the same level of aconitase activity as CTRL (97%; Figure 3(e)) and increased mitochondrial superoxide dismutase (SOD) by 36% compared to the PAH group (Figure 3(g)), which is a direct target of SIRT3.

3.4. RES Decreases the Acetylation of CypD

To evaluate the extent of sirtuin activation by RES, the mitochondrial protein acetylation profile, SIRT3 expression, and acetylation of CypD were assessed. In Figure 4(a), the protein acetylation profiles of isolated mitochondria show a 59% increase in acetylated proteins in the PAH group, including a threefold increase in CypD acetylation (Figure 4(c)). Protein acetylation was decreased by 13% in the PAH-RES group ( vs. PAH); however, SIRT3 was 96% overexpressed (Figure 4(b)). Importantly, CypD was a critical component of mitochondria permeability transitioning, as shown by the significant decrease of 51% (, vs. PAH) in acetylation in the PAH-RES group (Figure 4(c)), indicating the importance of SIRT3 in reducing mitochondrial permeability transitioning. There were no significant between-group differences in SIRT1 gene expression (; ; PAH+mRNA/HPRT), while SIRT5 decreased in both the PAH and PAH+RES groups (; ; PAH+mRNA/HPRT).

4. Discussion

The cardiovascular protective actions of RES in PAH have been reported in RV function [16, 38]; however, the mechanisms involved have not been fully described. According to our results, PAH causes an energetic dysfunction in the RV myocyte by promoting the opening of the mPTP due to CypD hyperacetylation. The decreased energy supply impairs the highly energy-demanding processes involved in myocyte functions, such as cellular relaxation, by hampering SERCA activity and delaying myofibrils’ unbinding. Treating this model with RES stimulates and overexpresses SIRT3, which prevents mPTP opening by acting directly on CypD deacetylation. Preserving cellular energetics also preserves myocyte contraction and relaxation.

4.1. RES Improves Cell Relaxation and SERCA Activity

Intracellular Ca2+ oscillations orchestrate cell contraction-relaxation cycle during Ca2+ transient, since cytosolic Ca2+ interacts with troponin C allowing actin-myosin interaction.

RV myocyte functioning was evaluated using confocal microscopy by assessing intracellular Ca2+ signaling and cell shortening. Characterization of the cellular contraction-relaxation cycle showed that PAH has a negative impact on the overall contraction-relaxation dynamic. Regardless, no alterations in SR Ca2+ release synchronicity during Ca2+ transient; it takes longer to accomplish maximal shortening. Treating PAH with RES decreased time to maximal shortening possibly by increased myofilament Ca2+ sensitivity [39, 40]; however, it does not fully normalize this parameter. Interestingly, relaxation dynamics showed the most significant changes. PAH considerably prolongs cell relaxation, while PAH under RES treatment keeps the relaxation rate similar to the CTRL group, a finding that has not been previously reported.

Accordingly, major alteration in intracellular Ca2+ transient caused by PAH was a decreased SERCA activity caused by a decreased SERCA/PLB ratio. However, both increased [41] and decreased [42] SERCA activities have been reported, as well as no change in SERCA and PLB expression [41]. Although RES treatment did not change the SERCA/PLB ratio, it did increase intracellular Ca2+ removal, thus SERCA activity.

This behavior was replicated after stimulating the β-AR, a highly energy-demanding condition [43, 44]. PAH showed the highest transient amplitude but the lowest cell shortening, while RES preserved the proportionality of Ca2+ released and cell contraction.

This effect might be related to a mismatch in the ECEC since it has been documented that creatine kinase (CK) expression is diminished in failing RV caused by PAH due to a decreased ATP supply [21, 45, 46]. Failing to meet the energetic demand, myofilament cross-bridge cycling is inhibited in finding shorter sarcomere lengths [21], compromising myocyte function. In this regard, the preservation of ATP production by RES preserves CK activity and an efficient ATP supply to SERCA, displaying improved cell contraction and relaxation.

Additionally, PAH did not modify Ca2+ spark frequency, indicating intact RyR activity [47], unlike previous reports [41, 42]. RES treatment also showed no changes in spark frequency and amplitude.

4.2. RES Preserves Mitochondrial Functioning and Integrity

Since major alterations caused by PAH reside among highly energy-dependent mechanisms, cell excitation and contraction must be tightly linked to the energy supply to ensure the proper functioning of the myocyte as a whole in an ECEC process. Since mitochondrial dysfunction has been identified as one of the mechanisms underlying heart failure [18, 19, 22, 46], mitochondrial activity was evaluated in this model. In isolated myocytes, PAH compromises ATP production by decreasing ; the electrochemical force needed for ATP production, decreasing the oxidative phosphorylation rate (state 3). Decreased phosphorylation response have been reported in RV by PAH [4850]. The cardioprotective effects of RES on mitochondria have been described in several models [5153]. Similarly, RES treatment preserved and respiratory chain activity in PAH. Even though the results obtained by mitochondrial respiration and fragility are evident when stimulating complex II, these same aspects have yet to be evaluated under NADH-dependent respiration.

Mitochondrial function preservation by RES in PAH could be related to decrease mitochondrial fragility. The loss of mitochondrial integrity by mPTP formation has been described as a main contributor to ventricular dysfunction in the right and left ventricles [22, 54, 55]. Most importantly, preventing mPTP opening using CsA has been shown to reduce RV dysfunction in PAH [22]. Mitochondrial Ca2+ overload in PAH, complemented by an increased oxidative environment within the mitochondria, makes them more prone to permeability transition [54, 56]; however, unlike other reports [57], no critical signs of proteins being modified by oxidative stress were observed, indicating that the antioxidant system is capable of managing oxidative stress caused by PAH in this model.

Although evident impairment in was found in this study, outright evidence from reduced cellular bioenergetics in this PAH model would directly measure ATP levels and evaluate the phosphocreatine system. However, it is well established that the ATP phosphorylation is particularly sensitive to decreases of mitochondrial membrane potential; for every 14 mV decrease in proton-motive force (equivalent to ), the ATP/ADP ratio decreases by 10-fold [58]. Also, the mitochondrial membrane potential has been described as a crucial factor to generate rotational torque by the nanomotor [59, 60]. Thus, a decrease in this electrochemical force may impede ATP production. In this regard, the integrity of in PAH+RES RV myocytes suggests a capable, energetic system to sustain the cardiac ECC.

4.3. RES Promotes the Deacetylation of CypD by SIRT3 Overexpression

One of the mechanisms through which RES bestows its protective effects is the activation of deacetylases. In pulmonary arterial smooth muscle cells (PASMC), the protective effect of RES has been linked to expression and activity modulation of the cytosolic deacetylase SIRT1 [61, 62]. Similarly, an increase in acetylated proteins was found in PAH RV myocytes [16, 38], and the cardiac protection of RES through SIRT1 activation has been reported in different conditions [38, 6365]. Since PAH’s effect is on mitochondrial function and activity, the expression of SIRT3 and mitochondrial acetylome were evaluated to determine the extent of its involvement.

The mitochondrial deacetylase SIRT3, which regulates mitochondrial function [6669], is modulated by RES [12], and the rs11246020 polymorphism, associated with a ~30% loss of function, has been found to be overrepresented in patients with idiopathic PAH [25]. PAH showed an increase in the protein acetylation profile from mitochondria, similar to reports in PASMC [25]. RES treatment increased SIRT3 expression almost 3.5-fold; however, the acetylation profile did not decrease significantly from PAH levels. Regardless of this discrepancy, an important direct target of SIRT3, cyclophilin D (CypD), decreased by almost half its hyperacetylation, diminishing the mitochondria’s proneness to mPTP opening [15, 23], thus preserving the cellular energetic state (Figure 5).

Furthermore, SIRT3 activity has been linked to the prevention of myocardial dysfunction. Treatment with honokiol, a potent SIRT3 activator, prevents and reverses ventricular hypertrophy [70] and preserves mitochondrial integrity and energetic capability [70, 71]. The mechanisms involved still need to be elucidated; however, it has been found that SIRT3 prevents mitochondrial Ca2+ overload by regulating mitochondrial Ca2+ uptake, regulating the expression of mitochondrial Ca2+ uniporter and its main regulator MICU1. These data are relevant because it was established that MCU and the MICU1 promoter are regulated by SIRT3-dependent histone acetylation [72]. However, no change in MCU gene expression was found in this model.

While SIRT3 activity has been identified as being involved in cardiovascular protection [7377], it is not the only mechanism through which RES acts as a cardioprotective agent. Other sirtuins and enzymes, such as SIRT1, SIRT5, and AMPK [5, 6, 78], contribute to modulating the activation or repression of a wide range of cellular components [5, 6, 78]. Furthermore, PAH pathogenesis is not caused by a single modification; according to the widely accepted “multiple-hit” hypothesis: inflammation, genetic determinants, and environmental factors are needed to develop the disease [79, 80].

Another important mechanism involved in modulating mitochondrial functioning that we did not explore thoroughly in this study is mitochondrial dynamics. The deacetylation of OPA1 by SIRT3 has been described as a regulator of mitochondrial dynamics and plays a role in maintaining a competent mitochondrial population in the heart when it is under pathological stress [81]. While previous reports did not find changes in the gene expression of proteins involved in mitochondrial dynamics and biogenesis in PAH [82], it has been reported that RES promotes mitochondrial fission [83]. This phenomenon is needed to preserve mitochondrial function [84] and may be involved in preservation by RES in this model. However, the implications of mitochondrial dynamics in the progression of RV failure still need to be addressed; this phenomenon could be an interesting area of research in the future to elucidate new therapeutic targets in PAH.

Although we found a strong relationship between preservation of mitochondrial function and CypD acetylation via SIRT3, loss and gain of function experiments can assess its definitive role in this model. The availability of deficient-SIRT3 mice faces the challenge of PHA model development, since it has been reported that mouse PAH models may not develop pulmonary hypertension, RV hypertrophy, and RV failure regardless pulmonary artery remodeling; besides, some of the models show spontaneous reverse of pulmonary hypertension once the inductor is not present [85, 86].

4.4. Clinical Implications

This study suggests that mitochondrial protection and cellular energetic preservation could be possible therapeutic targets to improve the PAH phenotype. The currently approved PAH medications decrease vascular remodeling by restoring the balance between vasoactive and vasodilator mediators [87]. However, researchers have begun to focus on mitochondrial disorders to develop new strategies. Molecules that prevent and reverse mitochondrial bioenergetic abnormalities in PASMC are being explored due to their ability to promote apoptosis, thus decreasing pulmonary vascular remodeling [8891] and, in RV fibroblasts, reducing cardiac fibrosis in PAH [92]. Unfortunately, cardioprotective effects on RV muscle cells have not been explored. Although RES’ usefulness in treating cardiovascular diseases has been observed as an overall beneficial effect in diverse clinical trials, further research is needed to ensure sustained effectiveness in patients since its major disadvantage is its poor bioavailability [93]. No published studies have evaluated RES use in PAH patients. Finally, ECEC disruption is a phenomenon found in the right and left heart failure. Describing the underlying mechanism and identifying shared targets may be useful to recognize therapeutic strategies that can help to improve heart failure prognosis and care.

5. Conclusions

The present work assessed the alterations in RV myocytes caused by PAH and RES’ protection. For the first time, we showed that the development of PAH causes a mismatch in the ECEC: compromised mitochondrial functioning and altered ATP synthesis resulted in deficient cell relaxation and disrupted cell contraction. RES protects mitochondria integrity by decreasing CypD hyperacetylation and increasing SIRT3 expression and activity, preventing mPTP opening, and preserving the . Maintaining cellular energetics preserves ECEC, ensuring the proper functioning of the myocyte as a whole. Understanding the mechanisms involved in the protection that RES confers on the RV in PAH could facilitate the development of new adjuvant therapies that improve the daily lives of PAH patients.

Data Availability

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

Disclosure

This work was submitted in partial fulfilment of the requirements for the PhD degree (JBR) for the Doctorate in Biotechnology, Tecnológico de Monterrey.

Conflicts of Interest

The authors declare that there is no conflict of interest regarding the publication of this paper.

Acknowledgments

The authors wish to acknowledge the financial support of Tecnológico de Monterrey and a CONACYT doctoral fellowship (Grant 492122 to JBR). This work was supported by the CONACYT (Grants 256577 and 258197), Fronteras de la Ciencia (0682), and Ciencia Básica (A1-S-43883 (GGR)). Thanks are due to Dr. Edgar Acuña-Morín for their excellent technical support.

Supplementary Materials

Supplemental Table 1: qPCR primer sequences hypoxanthine phosphoribosyltransferase 1 (HPRT), Na+/Ca2+ exchanger (NCX), sirtuin 1 (Sirt1), sirtuin 5 (Sirt5), and mitochondria calcium uniplex (MCU). HPRT was used as a housekeeping gene. Supplementary Figure 1: heart and lung structural comparison between control animals and RES-treated control animals. Pooled data of muscularized arteries (A), luminal diameter (B), and occlusion (C) in the lung tissue (H&E, 10x). Bar graph depicting the myocyte area (D) in RV. Data was normalized to CTRL mean values. All data are presented as the . vs. CTRL calculated by a -test followed by the Mann–Whitney test. Supplementary Figure 2: characterization of RV myocytes Ca2+ transient in isolated RV myocytes. (A) Representative line scan images of Ca2+ transient before (baseline) and after β-adrenergic stimulation with 100 nM isoproterenol (ISO). Pooled data of Ca2+ transient amplitude (B), time to 50% decay (, C), and time to peak (D) (CTRL:cells and 4 animals; PAH:cells and 3-4 animals; PAH+RES:cells and 4 animals; baseline and ISO, respectively). (E) Percentage of maximal shortening before and after β-adrenergic stimulation (CTRL:cells and 1-4 animals; PAH:cells and 3-4 animals; PAH+RES:cells and 4 animals; baseline and ISO, respectively). Records were taken under 1 Hz pace. CTRL: control; PAH: pulmonary arterial hypertension; PAH+RES: PAH treated with resveratrol. All data are presented as the , unless otherwise stated. vs. respective CTRL, a vs. respective PAH, and b vs. respective basal, calculated by 1-way ANOVA. (Supplementary Materials)

References

  1. A. Hemnes, A. M. K. Rothman, A. J. Swift, and L. S. Zisman, “Role of biomarkers in evaluation, treatment and clinical studies of pulmonary arterial hypertension,” Pulmonary Circulation, vol. 10, no. 4, 2020. View at: Publisher Site | Google Scholar
  2. F. S. de Man, M. L. Handoko, and A. Vonk-Noordegraaf, “The unknown pathophysiological relevance of right ventricular hypertrophy in pulmonary arterial hypertension,” European Respiratory Journal, vol. 53, no. 4, 2019. View at: Publisher Site | Google Scholar
  3. N. Galiè, R. N. Channick, R. P. Frantz et al., “Risk stratification and medical therapy of pulmonary arterial hypertension,” European Respiratory Journal, vol. 53, no. 1, p. 1801889, 2019. View at: Publisher Site | Google Scholar
  4. A. Huertas, L. Tu, M. Humbert, and C. Guignabert, “Chronic inflammation within the vascular wall in pulmonary arterial hypertension: more than a spectator,” Cardiovascular Research, vol. 116, no. 5, pp. 885–893, 2020. View at: Publisher Site | Google Scholar
  5. S. Bradamante, L. Barenghi, and A. Villa, “Cardiovascular Protective Effects of Resveratrol,” Cardiovascular drug reviews, vol. 22, no. 3, pp. 169–188, 2004. View at: Publisher Site | Google Scholar
  6. S. S. Kulkarni and C. Cantó, “The molecular targets of resveratrol,” Biochimica et Biophysica Acta (BBA) - Molecular Basis of Disease, vol. 1852, no. 6, pp. 1114–1123, 2015. View at: Publisher Site | Google Scholar
  7. A. Sanches-Silva, L. Testai, S. F. Nabavi et al., “Therapeutic potential of polyphenols in cardiovascular diseases: regulation of mTOR signaling pathway,” Pharmacological Research, vol. 152, p. 104626, 2020. View at: Publisher Site | Google Scholar
  8. D. Bonnefont-Rousselot, “Resveratrol and cardiovascular diseases,” Nutrients, vol. 8, no. 5, p. 250, 2016. View at: Publisher Site | Google Scholar
  9. A. Csiszar, N. Labinskyy, S. Olson et al., “Resveratrol prevents monocrotaline-induced pulmonary hypertension in rats,” Hypertension, vol. 54, no. 3, pp. 668–675, 2009. View at: Publisher Site | Google Scholar
  10. R. K. Vella, C. Pullen, F. R. Coulson, and A. S. Fenning, “Resveratrol prevents cardiovascular complications in the SHR/STZ rat by reductions in oxidative stress and inflammation,” BioMed Research International, vol. 2015, Article ID 918123, 8 pages, 2015. View at: Publisher Site | Google Scholar
  11. M. M. Poulsen, K. Fjeldborg, M. J. Ornstrup, T. N. Kjær, M. K. Nøhr, and S. B. Pedersen, “Resveratrol and inflammation: challenges in translating pre-clinical findings to improved patient outcomes,” Biochimica et Biophysica Acta (BBA) - Molecular Basis of Disease, vol. 1852, no. 6, pp. 1124–1136, 2015. View at: Publisher Site | Google Scholar
  12. N. Treviño-Saldaña and G. García-Rivas, “Regulation of sirtuin-mediated protein deacetylation by cardioprotective phytochemicals,” Oxidative Medicine and Cellular Longevity, vol. 2017, Article ID 1750306, 16 pages, 2017. View at: Publisher Site | Google Scholar
  13. N. R. Sundaresan, M. Gupta, G. Kim, S. B. Rajamohan, A. Isbatan, and M. P. Gupta, “Sirt3 blocks the cardiac hypertrophic response by augmenting Foxo3a-dependent antioxidant defense mechanisms in mice,” The Journal of Clinical Investigation, vol. 119, no. 9, pp. 2758–2771, 2009. View at: Publisher Site | Google Scholar
  14. M. Kerr, J. J. Miller, D. Thapa et al., “Rescue of myocardial energetic dysfunction in diabetes through the correction of mitochondrial hyperacetylation by honokiol,” JCI insight, vol. 5, no. 17, 2020. View at: Publisher Site | Google Scholar
  15. E. C. Castillo, J. A. Morales, H. Chapoy-Villanueva et al., “Mitochondrial hyperacetylation in the failing hearts of obese patients mediated partly by a reduction in SIRT3: the involvement of the mitochondrial permeability transition pore,” Cellular Physiology and Biochemistry, vol. 53, no. 3, pp. 465–479, 2019. View at: Publisher Site | Google Scholar
  16. E. Vázquez-Garza, J. Bernal-Ramírez, C. Jerjes-Sánchez et al., “Resveratrol prevents right ventricle remodeling and dysfunction in monocrotaline-induced pulmonary arterial hypertension with a limited improvement in the lung vasculature,” Oxidative Medicine and Cellular Longevity, vol. 2020, Article ID 1841527, 13 pages, 2020. View at: Publisher Site | Google Scholar
  17. N. V. Shults, S. S. Kanovka, J. E. Ten Eyck, V. Rybka, and Y. J. Suzuki, “Ultrastructural changes of the right ventricular myocytes in pulmonary arterial hypertension,” Journal of the American Heart Association, vol. 8, no. 5, article e011227, 2019. View at: Publisher Site | Google Scholar
  18. F. Potus, C. Hindmarch, K. Dunham-Snary, J. Stafford, and S. Archer, “Transcriptomic signature of right ventricular failure in experimental pulmonary arterial hypertension: deep sequencing demonstrates mitochondrial, fibrotic, inflammatory and angiogenic abnormalities,” International Journal of Molecular Sciences, vol. 19, no. 9, 2018. View at: Publisher Site | Google Scholar
  19. L. Piao, Y.-H. Fang, V. J. J. Cadete et al., “The inhibition of pyruvate dehydrogenase kinase improves impaired cardiac function and electrical remodeling in two models of right ventricular hypertrophy: resuscitating the hibernating right ventricle,” Journal of Molecular Medicine (Berlin, Germany), vol. 88, no. 1, pp. 47–60, 2010. View at: Publisher Site | Google Scholar
  20. L. Piao, G. Marsboom, and S. L. Archer, “Mitochondrial metabolic adaptation in right ventricular hypertrophy and failure,” Journal of Molecular Medicine (Berlin, Germany), vol. 88, no. 10, pp. 1011–1020, 2010. View at: Publisher Site | Google Scholar
  21. E. D. Fowler, D. Benoist, M. J. Drinkhill et al., “Decreased creatine kinase is linked to diastolic dysfunction in rats with right heart failure induced by pulmonary artery hypertension,” Journal of Molecular and Cellular Cardiology, vol. 86, pp. 1–8, 2015. View at: Publisher Site | Google Scholar
  22. D. S. Lee and Y. W. Jung, “Protective effect of right ventricular mitochondrial damage by cyclosporine A in monocrotaline-induced pulmonary hypertension,” Korean Circulation Journal, vol. 48, no. 12, pp. 1135–1144, 2018. View at: Publisher Site | Google Scholar
  23. A. V. Hafner, J. Dai, A. P. Gomes et al., “Regulation of the mPTP by SIRT3-mediated deacetylation of Cyp D at lysine 166 suppresses age-related cardiac hypertrophy,” Aging, vol. 2, no. 12, pp. 914–923, 2010. View at: Publisher Site | Google Scholar
  24. T. Bochaton, C. Crola-Da-Silva, B. Pillot et al., “Inhibition of myocardial reperfusion injury by ischemic postconditioning requires sirtuin 3-mediated deacetylation of cyclophilin D,” Journal of Molecular and Cellular Cardiology, vol. 84, pp. 61–69, 2015. View at: Publisher Site | Google Scholar
  25. R. Paulin, P. Dromparis, G. Sutendra et al., “Sirtuin 3 deficiency is associated with inhibited mitochondrial function and pulmonary arterial hypertension in rodents and humans,” Cell Metabolism, vol. 20, no. 5, pp. 827–839, 2014. View at: Publisher Site | Google Scholar
  26. J. R. Klinger, C. G. Elliott, D. J. Levine et al., “Therapy for pulmonary arterial hypertension in adults: update of the CHEST guideline and expert panel report,” Chest, vol. 155, no. 3, pp. 565–586, 2019. View at: Publisher Site | Google Scholar
  27. D. Santos-Ribeiro, P. Mendes-Ferreira, C. Maia-Rocha, R. Adão, A. F. Leite-Moreira, and C. Brás-Silva, “Hypertension arterielle pulmonaire : connaissances de base pour les cliniciens,” Archives of Cardiovascular Diseases, vol. 109, no. 10, pp. 550–561, 2016. View at: Publisher Site | Google Scholar
  28. C. E. Guerrero-Beltrán, J. Bernal-Ramírez, O. Lozano et al., “Silica nanoparticles induce cardiotoxicity interfering with energetic status and Ca2+ handling in adult rat cardiomyocytes,” American Journal of Physiology-Heart and Circulatory Physiology, vol. 312, no. 4, pp. H645–H661, 2017. View at: Publisher Site | Google Scholar
  29. P. Pérez-Treviño, J. Sepúlveda-Leal, and J. Altamirano, “Simultaneous assessment of calcium handling and contractility dynamics in isolated ventricular myocytes of a rat model of post-acute isoproterenol- induced cardiomyopathy,” Cell Calcium, vol. 86, p. 102138, 2020. View at: Publisher Site | Google Scholar
  30. E. Fernández-Sada, C. Silva-Platas, C. A. Villegas et al., “Cardiac responses to β-adrenoceptor stimulation is partly dependent on mitochondrial calcium uniporter activity,” British Journal of Pharmacology, vol. 171, no. 18, pp. 4207–4221, 2014. View at: Publisher Site | Google Scholar
  31. E. Picht, A. V. Zima, L. A. Blatter, and D. M. Bers, “SparkMaster: automated calcium spark analysis with ImageJ,” American Journal of Physiology. Cell Physiology, vol. 293, no. 3, pp. C1073–C1081, 2007. View at: Publisher Site | Google Scholar
  32. C. Silva-Platas, C. E. Guerrero-Beltrán, M. Carrancá et al., “Antineoplastic copper coordinated complexes (Casiopeinas) uncouple oxidative phosphorylation and induce mitochondrial permeability transition in cardiac mitochondria and cardiomyocytes,” Journal of Bioenergetics and Biomembranes, vol. 48, no. 1, pp. 43–54, 2016. View at: Publisher Site | Google Scholar
  33. G. de Jesús García-Rivas, A. Guerrero-Hernández, G. Guerrero-Serna, J. S. Rodríguez-Zavala, and C. Zazueta, “Inhibition of the mitochondrial calcium uniporter by the oxo-bridged dinuclear ruthenium amine complex (Ru360) prevents from irreversible injury in postischemic rat heart,” The FEBS Journal, vol. 272, no. 13, pp. 3477–3488, 2005. View at: Publisher Site | Google Scholar
  34. H. Chapoy-Villanueva, C. Silva-Platas, A. K. Gutiérrez-Rodríguez et al., “Changes in the stoichiometry of uniplex decrease mitochondrial calcium overload and contribute to tolerance of cardiac ischemia/reperfusion injury in hypothyroidism,” Thyroid, vol. 29, no. 12, pp. 1755–1764, 2019. View at: Publisher Site | Google Scholar
  35. N. García, J. J. García, F. Correa, and E. Chávez, “The permeability transition pore as a pathway for the release of mitochondrial DNA,” Life Sciences, vol. 76, no. 24, pp. 2873–2880, 2005. View at: Publisher Site | Google Scholar
  36. J. E. Vela-Guajardo, P. Pérez-Treviño, I. Rivera-Álvarez, F. A. González-Mondellini, J. Altamirano, and N. García, “The 8-oxo-deoxyguanosine glycosylase increases its migration to mitochondria in compensated cardiac hypertrophy,” Journal of the American Society of Hypertension, vol. 11, no. 10, pp. 660–672, 2017. View at: Publisher Site | Google Scholar
  37. R. Nogueira-Ferreira, R. Vitorino, R. Ferreira, and T. Henriques-Coelho, “Exploring the monocrotaline animal model for the study of pulmonary arterial hypertension: a network approach,” Pulmonary Pharmacology & Therapeutics, vol. 35, pp. 8–16, 2015. View at: Publisher Site | Google Scholar
  38. P. Chelladurai, O. Boucherat, K. Stenmark et al., “Targeting histone acetylation in pulmonary hypertension and right ventricular hypertrophy,” British Journal of Pharmacology, vol. 178, no. 1, pp. 54–71, 2021. View at: Publisher Site | Google Scholar
  39. R. Liew, M. A. Stagg, K. T. MacLeod, and P. Collins, “The red wine polyphenol, resveratrol, exerts acute direct actions on guinea- pig ventricular myocytes,” European Journal of Pharmacology, vol. 519, no. 1-2, pp. 1–8, 2005. View at: Publisher Site | Google Scholar
  40. S. E. Pineda-Sanabria, I. M. Robertson, and B. D. Sykes, “Structure of trans-resveratrol in complex with the cardiac regulatory protein troponin C,” Biochemistry, vol. 50, no. 8, pp. 1309–1320, 2011. View at: Publisher Site | Google Scholar
  41. J. Sabourin, A. Boet, C. Rucker-Martin et al., “Ca2+ handling remodeling and STIM1L/Orai1/TRPC1/TRPC4 upregulation in monocrotaline-induced right ventricular hypertrophy,” Journal of Molecular and Cellular Cardiology, vol. 118, pp. 208–224, 2018. View at: Publisher Site | Google Scholar
  42. D. Benoist, R. Stones, M. J. Drinkhill et al., “Cardiac arrhythmia mechanisms in rats with heart failure induced by pulmonary hypertension,” American Journal of Physiology-Heart and Circulatory Physiology, vol. 302, no. 11, pp. H2381–H2395, 2012. View at: Publisher Site | Google Scholar
  43. Y. Fu, R. E. Westenbroek, T. Scheuer, and W. A. Catterall, “Phosphorylation sites required for regulation of cardiac calcium channels in the fight-or-flight response,” Proceedings of the National Academy of Sciences of the United States of America, vol. 110, no. 48, pp. 19621–19626, 2013. View at: Publisher Site | Google Scholar
  44. A. E. Messer and S. B. Marston, “Investigating the role of uncoupling of troponin I phosphorylation from changes in myofibrillar Ca2+-sensitivity in the pathogenesis of cardiomyopathy,” Frontiers in Physiology, vol. 5, p. 315, 2014. View at: Publisher Site | Google Scholar
  45. E. D. Fowler, M. J. Drinkhill, R. Stones, and E. White, “Diastolic dysfunction in pulmonary artery hypertension: Creatine kinase and the potential therapeutic benefit of beta-blockers,” Clinical and Experimental Pharmacology and Physiology, vol. 45, no. 4, pp. 384–389, 2018. View at: Publisher Site | Google Scholar
  46. E. D. Fowler, D. Hauton, J. Boyle, S. Egginton, D. S. Steele, and E. White, “Energy metabolism in the failing right ventricle : limitations of oxygen delivery and the creatine kinase system,” International Journal of Molecular Sciences, vol. 20, no. 8, 2019. View at: Publisher Site | Google Scholar
  47. A. Kushnir, B. Wajsberg, and A. R. Marks, “Ryanodine receptor dysfunction in human disorders,” Biochimica et Biophysica Acta (BBA) - Molecular Cell Researchs, vol. 1865, no. 11, pp. 1687–1697, 2018. View at: Publisher Site | Google Scholar
  48. K. A. Cottrill and S. Y. Chan, “Metabolic dysfunction in pulmonary hypertension: the expanding relevance of the Warburg effect,” European Journal of Clinical Investigation, vol. 43, no. 8, pp. 855–865, 2013. View at: Publisher Site | Google Scholar
  49. J. Gomez-Arroyo, S. Mizuno, K. Szczepanek et al., “Metabolic gene remodeling and mitochondrial dysfunction in failing right ventricular hypertrophy secondary to pulmonary arterial hypertension,” Circulation. Heart Failure, vol. 6, no. 1, pp. 136–144, 2013. View at: Publisher Site | Google Scholar
  50. A. Vonk-Noordegraaf, F. Haddad, K. M. Chin et al., “Right heart adaptation to pulmonary arterial hypertension: physiology and pathobiology,” Journal of the American College of Cardiology, vol. 62, no. 25, pp. D22–D33, 2013. View at: Publisher Site | Google Scholar
  51. L. C. Thuc, Y. Teshima, N. Takahashi et al., “Inhibition of Na(+)-H(+) exchange as a mechanism of rapid cardioprotection by resveratrol,” British Journal of Pharmacology, vol. 166, no. 6, pp. 1745–1755, 2012. View at: Publisher Site | Google Scholar
  52. M. M. Sung, S. K. Das, J. Levasseur et al., “Resveratrol treatment of mice with pressure-overload-induced heart failure improves diastolic function and cardiac energy metabolism,” Circulation. Heart Failure, vol. 8, no. 1, pp. 128–137, 2015. View at: Publisher Site | Google Scholar
  53. T. Li, L. Chen, Y. Yu, B. Yang, P. Li, and X.-Q. Tan, “Resveratrol alleviates hypoxia/reoxygenation injury‑induced mitochondrial oxidative stress in cardiomyocytes,” Molecular Medicine Reports, vol. 19, no. 4, pp. 2774–2780, 2019. View at: Publisher Site | Google Scholar
  54. A. Riojas-Hernández, J. Bernal-Ramírez, D. Rodríguez-Mier et al., “Enhanced oxidative stress sensitizes the mitochondrial permeability transition pore to opening in heart from Zucker Fa/fa rats with type 2 diabetes,” Life Sciences, vol. 141, pp. 32–43, 2015. View at: Publisher Site | Google Scholar
  55. F. Ahmad, A. P. Singh, D. Tomar et al., “Cardiomyocyte-GSK-3α promotes mPTP opening and heart failure in mice with chronic pressure overload,” Journal of Molecular and Cellular Cardiology, vol. 130, pp. 65–75, 2019. View at: Publisher Site | Google Scholar
  56. R. Endlicher, Z. Drahota, and Z. Červinková, “In vitro and in vivo activation of mitochondrial membrane permeability transition pore using triiodothyronine,” Physiological Research, vol. 65, no. 2, pp. 321–331, 2016. View at: Publisher Site | Google Scholar
  57. N. L. Jernigan, J. S. Naik, L. Weise-Cross et al., “Contribution of reactive oxygen species to the pathogenesis of pulmonary arterial hypertension,” PLoS One, vol. 12, no. 6, article e0180455, 2017. View at: Publisher Site | Google Scholar
  58. D. G. Nicholls, “Mitochondrial membrane potential and aging,” Aging Cell, vol. 3, no. 1, pp. 35–40, 2004. View at: Publisher Site | Google Scholar
  59. P. Dimroth, G. Kaim, and U. Matthey, “Crucial role of the membrane potential for ATP synthesis by F (1) F (o) ATP synthases,” The Journal of Experimental Biology, vol. 203, no. 1, pp. 51–59, 2000. View at: Publisher Site | Google Scholar
  60. D. Stock, C. Gibbons, I. Arechaga, A. G. Leslie, and J. E. Walker, “The rotary mechanism of ATP synthase,” Current Opinion in Structural Biology, vol. 10, no. 6, pp. 672–679, 2000. View at: Publisher Site | Google Scholar
  61. S. Zhou, M.-T. Li, Y.-Y. Jia et al., “Regulation of Cell Cycle Regulators by SIRT1 Contributes to Resveratrol- Mediated Prevention of Pulmonary Arterial Hypertension,” BioMed Research International, vol. 2015, Article ID 762349, 14 pages, 2015. View at: Publisher Site | Google Scholar
  62. L. Yu, Y. Tu, X. Jia et al., “Resveratrol protects against pulmonary arterial hypertension in rats via activation of silent information regulator 1,” Cellular Physiology and Biochemistry, vol. 42, no. 1, pp. 55–67, 2017. View at: Publisher Site | Google Scholar
  63. S. Ma, J. Feng, R. Zhang et al., “SIRT1 activation by resveratrol alleviates cardiac dysfunction via mitochondrial regulation in diabetic cardiomyopathy mice,” Oxidative Medicine and Cellular Longevity, vol. 2017, Article ID 4602715, 15 pages, 2017. View at: Publisher Site | Google Scholar
  64. N. Fourny, C. Lan, E. Seree, M. Bernard, and M. Desrois, “Protective effect of resveratrol against ischemia-reperfusion injury via enhanced high energy compounds and eNOS-SIRT1 expression in type 2 diabetic female rat heart,” Nutrients, vol. 11, no. 1, 2019. View at: Publisher Site | Google Scholar
  65. Z.-H. Liu, Y. Zhang, X. Wang et al., “SIRT1 activation attenuates cardiac fibrosis by endothelial-to-mesenchymal transition,” Biomedicine & Pharmacotherapy, vol. 118, p. 109227, 2019. View at: Publisher Site | Google Scholar
  66. D. B. Lombard, F. W. Alt, H.-L. Cheng et al., “Mammalian Sir 2 homolog SIRT3 regulates global mitochondrial lysine acetylation,” Molecular and Cellular Biology, vol. 27, no. 24, pp. 8807–8814, 2007. View at: Publisher Site | Google Scholar
  67. S. Zhao, W. Xu, W. Jiang et al., “Regulation of cellular metabolism by protein lysine acetylation,” Science, vol. 327, no. 5968, pp. 1000–1004, 2010. View at: Publisher Site | Google Scholar
  68. L. W. S. Finley, W. Haas, V. Desquiret-Dumas et al., “Succinate dehydrogenase is a direct target of sirtuin 3 deacetylase activity,” PLoS One, vol. 6, no. 8, article e23295, 2011. View at: Publisher Site | Google Scholar
  69. M. D. Hirschey, T. Shimazu, E. Jing et al., “SIRT3 deficiency and mitochondrial protein hyperacetylation accelerate the development of the metabolic syndrome,” Molecular Cell, vol. 44, no. 2, pp. 177–190, 2011. View at: Publisher Site | Google Scholar
  70. V. B. Pillai, S. Samant, N. R. Sundaresan et al., “Honokiol blocks and reverses cardiac hypertrophy in mice by activating mitochondrial Sirt3,” Nature Communications, vol. 6, no. 1, 2015. View at: Publisher Site | Google Scholar
  71. V. B. Pillai, A. Kanwal, Y. H. Fang et al., “Honokiol, an activator of Sirtuin-3 (SIRT3) preserves mitochondria and protects the heart from doxorubicin-induced cardiomyopathy in mice,” Oncotarget, vol. 8, no. 21, pp. 34082–34098, 2017. View at: Publisher Site | Google Scholar
  72. P. Gao, Y. Jiang, H. Wu et al., “Inhibition of mitochondrial calcium overload by SIRT3 prevents obesity-or age-related whitening of brown adipose tissue,” Diabetes, vol. 69, no. 2, pp. 165–180, 2020. View at: Publisher Site | Google Scholar
  73. A. Benigni, P. Cassis, S. Conti et al., “Sirt3deficiency shortens life span and impairs cardiac mitochondrial function rescued byOpa1gene transfer,” Antioxidants & Redox Signaling, vol. 31, no. 17, pp. 1255–1271, 2019. View at: Publisher Site | Google Scholar
  74. S. Wang, Z. Zhao, Y. Fan et al., “Mst1 inhibits Sirt3 expression and contributes to diabetic cardiomyopathy through inhibiting Parkin-dependent mitophagy,” Biochimica et Biophysica Acta - Molecular Basis of Disease, vol. 1865, no. 7, pp. 1905–1914, 2019. View at: Publisher Site | Google Scholar
  75. A. E. Dikalova, A. Pandey, L. Xiao et al., “Mitochondrial deacetylase Sirt 3 reduces vascular dysfunction and hypertension while Sirt 3 depletion in essential hypertension is linked to vascular inflammation and oxidative stress,” Circulation Research, vol. 126, no. 4, pp. 439–452, 2020. View at: Publisher Site | Google Scholar
  76. X. Palomer, M. S. Román-Azcona, J. Pizarro-Delgado et al., “SIRT3-mediated inhibition of FOS through histone H3 deacetylation prevents cardiac fibrosis and inflammation,” Signal Transduction and Targeted Therapy, vol. 5, no. 1, p. 14, 2020. View at: Publisher Site | Google Scholar
  77. Z. Zhu, H. Li, W. Chen, Y. Cui, A. Huang, and X. Qi, “Perindopril improves cardiac function by enhancing the expression of SIRT3 and PGC-1α in a rat model of isoproterenol-induced cardiomyopathy,” Frontiers in Pharmacology, vol. 11, p. 94, 2020. View at: Publisher Site | Google Scholar
  78. A. McCalley, S. Kaja, A. J. Payne, and P. Koulen, “Resveratrol and calcium signaling: molecular mechanisms and clinical relevance,” Molecules, vol. 19, no. 6, pp. 7327–7340, 2014. View at: Publisher Site | Google Scholar
  79. R. Souza, C. Jardim, and M. Humbert, “Idiopathic pulmonary arterial hypertension,” Seminars in Respiratory and Critical Care Medicine, vol. 34, no. 5, pp. 560–567, 2013. View at: Publisher Site | Google Scholar
  80. R. Paulin and E. D. Michelakis, “The metabolic theory of pulmonary arterial hypertension,” Circulation Research, vol. 115, no. 1, pp. 148–164, 2014. View at: Publisher Site | Google Scholar
  81. S. A. Samant, H. J. Zhang, Z. Hong et al., “SIRT3 deacetylates and activates OPA1 to regulate mitochondrial dynamics during stress,” Molecular and Cellular Biology, vol. 34, no. 5, pp. 807–819, 2014. View at: Publisher Site | Google Scholar
  82. D. R. Bruns, R. D. Brown, K. R. Stenmark, P. M. Buttrick, and L. A. Walker, “Mitochondrial integrity in a neonatal bovine model of right ventricular dysfunction,” American Journal of Physiology. Lung Cellular and Molecular Physiology, vol. 308, no. 2, pp. L158–L167, 2015. View at: Publisher Site | Google Scholar
  83. X. Ren, L. Chen, J. Xie et al., “Resveratrol ameliorates mitochondrial elongation via Drp1/Parkin/PINK1 signaling in senescent-like cardiomyocytes,” Oxidative Medicine and Cellular Longevity, vol. 2017, Article ID 4175353, 20 pages, 2017. View at: Publisher Site | Google Scholar
  84. S. Pickles, P. Vigie, and R. J. Youle, “Mitophagy and quality control mechanisms in mitochondrial maintenance,” Current Biology, vol. 28, no. 4, pp. R170–R185, 2018. View at: Publisher Site | Google Scholar
  85. J. Gomez-Arroyo, S. J. Saleem, S. Mizuno et al., “A brief overview of mouse models of pulmonary arterial hypertension: problems and prospects,” American Journal of Physiology. Lung Cellular and Molecular Physiology, vol. 302, no. 10, pp. L977–L991, 2012. View at: Publisher Site | Google Scholar
  86. B. L. Carman, D. N. Predescu, R. Machado, and S. A. Predescu, “Plexiform arteriopathy in rodent models of pulmonary arterial hypertension,” The American Journal of Pathology, vol. 189, no. 6, pp. 1133–1144, 2019. View at: Publisher Site | Google Scholar
  87. M. Bisserier, N. Pradhan, and L. Hadri, “Current and emerging therapeutic approaches to pulmonary hypertension,” Reviews in Cardiovascular Medicine, vol. 21, no. 2, pp. 163–179, 2020. View at: Publisher Site | Google Scholar
  88. B. Li, Y. Zhu, Q. Sun et al., “Reversal of the Warburg effect with DCA in PDGF-treated human PASMC is potentiated by pyruvate dehydrogenase kinase-1 inhibition mediated through blocking Akt/GSK-3β signalling,” International Journal of Molecular Medicine, vol. 42, no. 3, pp. 1391–1400, 2018. View at: Publisher Site | Google Scholar
  89. M. S. McMurtry, S. Bonnet, X. Wu et al., “Dichloroacetate prevents and reverses pulmonary hypertension by inducing pulmonary artery smooth muscle cell apoptosis,” Circulation Research, vol. 95, no. 8, pp. 830–840, 2004. View at: Publisher Site | Google Scholar
  90. E. D. Michelakis, V. Gurtu, L. Webster et al., “Inhibition of pyruvate dehydrogenase kinase improves pulmonary arterial hypertension in genetically susceptible patients,” Science Translational Medicine, vol. 9, no. 413, 2017. View at: Publisher Site | Google Scholar
  91. R. Kurosawa, K. Satoh, N. Kikuchi et al., “Identification of celastramycin as a novel therapeutic agent for pulmonary arterial hypertension,” Circulation Research, vol. 125, no. 3, pp. 309–327, 2019. View at: Publisher Site | Google Scholar
  92. L. Tian, D. Wu, A. Dasgupta et al., “Epigenetic metabolic reprogramming of right ventricular fibroblasts in pulmonary arterial hypertension: a pyruvate dehydrogenase kinase-dependent shift in mitochondrial metabolism promotes right ventricular fibrosis,” Circulation Research, vol. 126, no. 12, pp. 1723–1745, 2020. View at: Publisher Site | Google Scholar
  93. A. Y. Berman, R. A. Motechin, M. Y. Wiesenfeld, and M. K. Holz, “The therapeutic potential of resveratrol: a review of clinical trials,” NPJ Precision Oncology, vol. 1, no. 1, 2017. View at: Publisher Site | Google Scholar

Copyright © 2021 Judith Bernal-Ramírez 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.

Related articles

No related content is available yet for this article.
 PDF Download Citation Citation
 Download other formatsMore
 Order printed copiesOrder
Views413
Downloads414
Citations

Related articles

No related content is available yet for this article.

Article of the Year Award: Outstanding research contributions of 2021, as selected by our Chief Editors. Read the winning articles.