Ketone Body <i>β</i>-Hydroxybutyrate Prevents Myocardial Oxidative Stress in Septic Cardiomyopathy

Ji, Liwei; He, Qinqin; Liu, Yinghai; Deng, Yan; Xie, Maodi; Luo, Kaiteng; Cai, Xintian; Zuo, Yunxia; Wu, Wei; Li, Qian; Zhou, Ronghua; Li, Tao

doi:https://doi.org/10.1155/2022/2513837

Oxidative Medicine and Cellular Longevity

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Mitochondrial Dysfunction and Oxidative Stress in Cardiovascular Diseases

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Research Article | Open Access

Volume 2022 | Article ID 2513837 | https://doi.org/10.1155/2022/2513837

Ketone Body β-Hydroxybutyrate Prevents Myocardial Oxidative Stress in Septic Cardiomyopathy

Liwei Ji,¹Qinqin He,¹Yinghai Liu,²Yan Deng,¹Maodi Xie,¹Kaiteng Luo,¹Xintian Cai,¹Yunxia Zuo,¹Wei Wu,²Qian Li,¹Ronghua Zhou,¹and Tao Li¹

Academic Editor: Abdur Rauf

Received15 Nov 2021

Revised27 Jan 2022

Accepted15 Feb 2022

Published18 Mar 2022

Abstract

Septic cardiomyopathy is a life-threatening complication of severe sepsis and septic shock. Oxidative stress and mitochondrial dysfunction have been identified as significant abnormalities in septic cardiomyopathy. However, specific treatments are rare. This study aims to investigate the impact of β-hydroxybutyrate (β-OHB) on septic cardiomyopathy and explore the underlying mechanism(s). We found that pretreatment of D-β-hydroxybutyrate-(R)-1,3 butanediol monoester (ketone ester, 3 mg/g body weight, once daily) by gavage for three days elevated the levels of ketone bodies, especially that of β-hydroxybutyrate (β-OHB) in the circulation and mouse hearts, which exerted a protective effect against lipopolysaccharide (LPS, 20 mg/kg)-induced septic cardiomyopathy in mice. In addition, an LPS-stimulated macrophage-conditioned medium (MCM) was used to mimic the pathological process of septic cardiomyopathy. Mechanistically, β-OHB alleviated myocardial oxidative stress and improved mitochondrial respiratory function through the antioxidant FoxO3a/MT2 pathway activated via histone deacetylase (HDAC) inhibition, which ultimately enhanced heart performance in septic cardiomyopathy. Our results, therefore, suggested an unappreciated critical role of β-OHB in septic heart protection as well as highlighted the potential of β-OHB as a simple remedy for the septic cardiomyopathy population.

1. Introduction

Sepsis is the leading cause of death among intensive care unit patients and is estimated to affect over 30 million people annually worldwide [1, 2]. Cardiac dysfunction caused by sepsis, which is defined as sepsis-induced cardiomyopathy, is an acute complication of severe sepsis and increases the mortality risk substantially [3, 4]. Septic cardiomyopathy is characterized by impaired left ventricular systolic and diastolic functions [5–7]. However, the pathogenesis of septic cardiomyopathy remains obscure [3, 8]. The treatment for this fatal condition remains largely supportive, and the therapeutic implications are uncertain [4, 9]. Hence, to manage the condition, it is imperative to explain the pathophysiological processes of septic cardiomyopathy and devise efficacious approaches.

Mitochondrial dysfunction and oxidative stress are increasingly recognized as the critical factors of septic myocardial injury [2, 8, 10]. The heart is an organ with high energy requirements and depends chiefly on mitochondrial oxidative phosphorylation (OXPHOS) [11, 12]. Mitochondria, the energy centers of cardiomyocytes, control cardiomyocyte metabolism and survival by constantly supplying ATP [13, 14]. Impaired mitochondrial respiratory function obstructs the energy supply and thus fails to support heart function in septic cardiomyopathy [7, 9, 15]. More importantly, mitochondria are a rich source of reactive oxygen species (ROS) in mammalian cells [14]. Under oxidative stress, increased ROS levels can damage mitochondrial membranes protein and DNA, thereby impairing the ability of the mitochondria to generate ATP [14, 16]. However, it is challenging to link these abnormalities to therapeutic strategies and relevant clinical outcomes. Therefore, antioxidant therapy targeting the mitochondrial function may facilitate the treatment of septic cardiomyopathy.

Several evidences highlight the crucial roles of ketone bodies in the pathophysiological progression of cardiovascular diseases, including heart failure, myocardial fibrosis, and vascular endothelial injury [17–20]. Ketone bodies include β-hydroxybutyrate (β-OHB), acetoacetate, and acetone [21]. In certain physiological states, such as fasting, starvation, and low-carbohydrate diets, ketone bodies become a significant source of overall energy and the substrate of mammalian metabolism in the extrahepatic tissues [21, 22]. In addition to acting as an alternative energy source, the ketone body β-OHB can serve as an endogenous histone deacetylase (HDAC) inhibitor, which is associated with increased global histone acetylation to initiate the transcription of antioxidant genes in response to oxidative stress [23]. Ketone ester (KE) could cause a rapid and significant increase in the blood D-β-OHB levels, and its production and commercialized has increased over the past decade. In light of the regulatory effects of β-OHB on oxidative stress, it is worthwhile to explore its cardioprotective effect and therapeutic potential in fatal septic cardiomyopathy based on redox homeostasis and mitochondrial performance.

In this study, we attempted to investigate the impacts of β-OHB on septic cardiomyopathy and elucidate the underlying mechanisms. By using animal models and cardiomyocytes to simulate the process of septic cardiomyopathy, the role of β-OHB as a HDAC inhibitor was demonstrated. β-OHB activated the antioxidant pathways to alleviate myocardial oxidative stress and improved the mitochondrial respiratory function, which ultimately enhanced the cardiac performance in septic cardiomyopathy.

2. Materials and Methods

2.1. Animal Care

All animal procedures were conducted in compliance with protocols approved by the Institutional Animal Care and Use Committee (IACUC) of the West China Hospital, Sichuan University, China (Protocol #20211406A). All animals were cared for in accordance with the recommendations provided in the Guide for the Care and Use of Laboratory Animals 8^th Edition. Healthy male C57BL/6 J mice aged 8 to 10 weeks were purchased from GemPharmatech Experimental Animal Centre, China. The mice were kept under specific pathogen-free (SPF) conditions at a constant temperature of 22°C on a 12 : 12 h light/dark cycle with free access to food and water. The septic mouse model was established as described previously [24, 25]. As female C57BL/6 J mice were reportedly resistant to cardiac injury in sepsis, we challenged male mice with a high dose of Escherichia coli lipopolysaccharide (LPS, 20 mg/kg, i.p., Sigma) to prepare septic cardiomyopathy models [5, 26]. The KE (D-β-hydroxybutyrate-R 1,3-butanediol monoester, KE) in this study is provided by a commercial drink from the T△S® Global company (Thame, UK) that contains 25 g KE in 59-mL purified water (pH~3.0) [27, 28]. Male C57BL/6 J mice aged 8–10 weeks were randomly categorized into three groups, namely, the control group (Control), LPS group (LPS), and pretreatment group. In the group, the mice received KE (3 mg/g body weight/day for three days) via oral gavage. In the control and LPS groups, the mice received an equivalent amount of saline for three days. Next, the LPS and groups mice were treated with LPS 30 min after administering the last dose of KE [28, 29]. After 6 h of LPS injection, the cardiac functions were assessed by 2-dimensional (2D) echocardiography. The hearts and blood collected from the mice in each group were used for further analyses. No death was recorded in this study within 6 h after the administration of LPS. No animals were intentionally excluded from the analyses.

2.2. Cell Culture

RAW264.7 murine macrophage cells were obtained from the American Type Culture Collection (ATCC; Rockville, MD, USA). The cells were cultured in Dulbecco’s Modified Eagle’s medium (DMEM; HyClone) (High Glucose) containing 1 g/L glucose, 4 mM glutamine, 110 mg/L sodium pyruvate supplemented with 10% (v/v) fetal bovine serum (FBS; Biological Industries), 100 U/mL penicillin, and 100 mg/mL streptomycin (both from HyClone Laboratories Inc.) under a humidified atmosphere of 5% CO₂ at 37°C. Referring to our previous protocol, RAW264.7 macrophage cells were treated with LPS (200 ng/mL, Sigma) for 6 h, and the medium was collected as macrophage-conditioned medium (MCM) [18]. The MCM was then stored for later use after filtration.

H9C2 rat myocardial cells were obtained from the American Type Culture Collection (ATCC; Rockville, MD, USA). The cells were cultured in high-glucose DMEM supplemented with 10% (v/v) FBS, 100 U/mL penicillin, and 100 mg/mL streptomycin under a humidified atmosphere of 5% CO₂ at 37°C. To determine the effects of β-OHB, the H9C2 cells were exposed to 10% MCM with or without 5 mM β-OHB for 24 h as described previously [18, 23]. N-acetylcysteine (NAC) (5 M, Sigma, A7250) was used as a nonspecific thiol antioxidant ROS scavenger. ITSA1 (10 μM, MedChemExpress), an activator of histone deacetylases, or entinostat (250 nM, MedChemExpress), a HDAC inhibitor, was used to induce histone acetylation in H9C2 cells exposed to MCM.

2.3. Measurement of β-OHB and Acetoacetic Acid (AcAc) Levels in the Plasma and Cardiac Tissues

After 6 h of LPS injection, the blood β-OHB concentrations were determined from tail blood samples with a ketone meter (Precision Xtra, Abbott). The β-OHB and AcAc levels in frozen cardiac tissues (5–10 mg) were measured by using the Ketone Body Assay Kit (#MAK134, Sigma) according to the supplier’s instructions.

2.4. Transthoracic Echocardiography

Transthoracic echocardiography was performed in mice using the Vevo 3100 High-Resolution In Vivo Imaging System instrument (Vevo 3100, FUJIFILM Visual Sonics, Canada) equipped with a 40-MHz MS550D scan probe. Mice were anesthetized with inhaled isoflurane (1% at 1 L/min oxygen flow), positioned supine on the animal-handling platform, with the chest area shaved and ultrasound coupling gel liberally applied to the left chest wall. Two-dimensional and M-mode echocardiographic images were recorded, and the ejection fraction (EF), fractional shortening (FS), and cardiac output (CO) were analyzed. All measurements were conducted in a blinded fashion.

2.5. Measurement of Creatine Kinase MB (CK-MB) and Lactate Dehydrogenase (LDH)

The blood samples were obtained via heart puncture after 6 h of LPS injection. The samples were centrifuged at 2500 rpm for 6 min at room temperature, and the plasma aliquots were collected for analysis. The concentrations of CK-MB and LDH in the plasma were measured using an automatic biochemical analyzer (BS-120; Mindray, China).

2.6. Histological Assessments

The mice hearts were arrested in diastole by KCl (30 mM), perfused with PBS through the heart, then fixed in 10% neutral buffered formalin for 24 h at 4°C. The hearts were embedded in paraffin and sectioned using a microtome. As for hematoxylin and eosin (H&E) staining, the left ventricle tissue sections (5-μm thickness) were stained with hematoxylin for 8 min, washed with running water, and then dipped in 1% hydrochloric acid in ethanol and 1% ammonium hydroxide, successively. Then, the sections were stained with eosin for 1 min, dehydrated with gradient ethanol, permeabilized with xylene, and mounted on slides with neutral balsam. The histological changes were observed by optical microscopy (Olympus, Tokyo, Japan) with 6 random fields of vision selected from each section.

2.7. Transmission Electron Microscopy

The left ventricular tissues were cut into small blocks (about 1 mm³), fixed with 2.5% glutaraldehyde and 2% paraformaldehyde in 0.1 M cacodylate buffer for 2 h, and then fixed with 1% cold osmium tetroxide for 2 h at 4°C. After dehydrating in gradient ethanol solutions (10 min/change) and embedded in Epon 812, the tissue blocks were cut into slices with a thickness of 60 nm using the Leica Cryostat System (EM UC7/FC7). The ultrathin sections were counterstained with 3% uranyl acetate and lead citrate. Then, mitochondrial ultrastructure was acquired using a transmission electron microscope (JEM-1400PLUS, JEOL, Japan). The images were analyzed by two pathologists in a blinded fashion.

2.8. Assessment of Mitochondrial Oxygen Consumption Rate (OCR)

The cardiac mitochondria were isolated using differential centrifugation described previously [30]. Briefly, freshly isolated hearts were rinsed with cold sucrose-containing mitochondrial isolation buffer, chopped into pieces, and then homogenized in mitochondrial isolation buffer using the Dounce homogenizer with Teflon pestle. Mitochondria were purified by sucrose density gradient centrifugation. The oxygen consumption rates (OCR) of cardiac mitochondria or cultured cells were measured using the Seahorse XFe24 Analyzer (seahorse, Agilent Technologies), as described previously [31]. Briefly, freshly isolated mitochondria were transferred to the XFe24 microplate filled with the mitochondria assay solution (MAS: 220 mM mannitol, 70 mM sucrose, 10 mM MgCl₂, 2 mM HEPES, 1 mM EGTA, 10 mM KH₂PO₄, and BSA 0.02% (w/v) at pH 7.2). The final volume was made up to 500 μL per well containing 10 mM pyruvate/5 mM malate (Sigma). OCR was measured at the baseline and after an sequential injection of ADP (4 mM, Sigma), oligomycin A (2.5 μg/mL, MCE), FCCP (trifluorocarbonyl cyanide phenylhydrazone, 4 μМ, MCE), and antimycin A (4 μМ, Sigma) at 37°C. For the cell OCR measurement, the H9C2 cells were maintained in a non-CO₂ incubator at 37°C for 1 h before starting the assay. The baseline OCR measurements were obtained first, followed by sequential injection of oligomycin A (5 μΜ final concentration, MCE), FCCP (3 μΜ final concentration, MCE), and Rotone/Antimycin A (1 μМ/1 μМ final concentration, Sigma) at 37°C. The respiratory rates are reported as oxygen flux per mass, and all readings are normalized to mitochondrial protein or cell number (pmolO₂/min/μg protein or 10000 cells).

2.9. Measurement of ROS and Superoxide Production

As measures of oxidative stress, the superoxide dismutase (SOD) activity and malondialdehyde (MDA) levels were detected in the cardiac tissues by using commercially available kits (Beyotime, China), according to the manufacturer’s recommendations. The protein carbonylation in the cardiac tissues was confirmed by measuring the protein carbonyl content using the OxyBlot Protein Oxidation Detection kit (Sigma). As for dihydroethidine (DHE) staining, the mouse cardiac tissues were embedded in the Tissue-Tek OCT compound (Sakura Finetek, Tokyo, Japan) and serially sectioned to 10-μm-thickness. The cryosections were stained with the superoxide-sensitive dye DHE (10 μM in 0.01% DMSO) and incubated for 30 min at 37°C in a humidified dark chamber. All sections were photographed under an inverted fluorescence microscope (IX83, Olympus, Japan). To detect mitochondrial superoxide production, H9C2 cells were incubated in a 6-well plate and stained with the Hoechst 33342 (Beyotime, #C1017) at 37°C for 20 min. After washing with PBS, H9C2 cells were incubated with the MitoSOX Red (5 μM, Thermo Fisher) for 10 min at 37°C. The nuclei were visualized at Ex: 346 nm, and the level of mitochondrial superoxide was visualized at Ex: 510 nm using the Olympus IX83 microscope. As for the quantitative detection of mitochondrial superoxide, the cells were incubated on a 96-well plate and stained with 2.5-μM MitoSOX Red at 37°C for 30 min, while the fluorescence intensity was quantified at 580 nm with a microplate reader (Biotek #21261610, USA). As for the MitoSOX flow cytometric analysis, H9C2 cells were incubated with 2.5 μM MitoSOX Red for 30 min at 37°C, washed with PBS, and resuspended in 200 μL ice-cold PBS. Flow cytometry analysis was immediately performed using the CytoFLEX flow cytometry (Beckman Coulter cytoFLEX, USA) equipped with Ex/Em: 510 nm/580 nm lasers. All of the abovementioned operations were performed without any light exposure.

2.9.1. Enzyme-Linked Immunosorbent Assay (ELISA)

ELISA kits of interleukin 1 beta (IL-1β, Elabscience, E-EL-R0012c), interleukin-6 receptor (IL-6, Elabscience, E-EL-M2453c), and tumor necrosis factor-alpha (TNF-α, Elabscience, E-MSEL-M0002) were employed to detect the levels of indicated inflammatory cytokines in LPS-stimulated MCM. All ELISA kits were purchased from Elabscience Biotechnology Co., Ltd (Wuhan, China). Briefly, the standards and samples were diluted, vortexed, and centrifuged before use. Next, IL-1β, IL-6, and TNF-α were analyzed by Sandwich ELISA kits following the manufacturer’s protocol. Inflammatory cytokines concentration was read immediately at 450 nm. The standard curve of each inflammatory cytokine was curve-fitted, and the unit of inflammatory cytokine was recorded in pictogram per milliliter.

2.10. RNA Isolation and Quantitative Real-Time PCR (qRT-PCR)

Total RNA was isolated from frozen left ventricular tissues or cultured cells with the TRIzol reagent (Thermo Fisher Scientific, Inc.). cDNA was synthesized with Omniscript reverse synthase and random hexamers according to the manufacturer’s guidelines (Vazyme Biotech). All primers were purchased from the TSINGKE Biosystems. qRT-PCR was performed with the SYBR green (Bio-Rad) under a cycling protocol (40 cycles) with 10-s denaturation (95°C), 20-s annealing (60°C), and 15-s extension (72°C). The relative mRNA expression of FoxO3a and MT2 were calculated by the ^ΔΔCt method, and the results were normalized to the GAPDH levels. The primers are described as follows:

FoxO3a_F, AGGACCTGCTCACTTCGGACTC;

FoxO3a_R,CAAGGCTGCTGGACTCACTCAAG;

MT2_F, ATGGATCCCAACTGCTCCTG;

MT2_R, CGACGCCCCTTTGCAGAT;

GAPDH_F, GAAGGTGAAGGTCGGAGTC;

GAPDH_R, GAAGATGGTGATGGGATTTC.

2.11. Acid Extraction of Histones

The frozen heart tissues were homogenized in an ice-cold Triton extraction buffer consisting with 0.5% Triton X-100, 2 mM phenylmethylsulfonyl fluoride (PMSF), 0.02% NaN₃, and 5 mM sodium butyrate. The lysates were mixed with vortexing for 10 min at 4°C and then centrifuged at 500 g for 10 min at 4°C. After washing twice in the Triton extraction buffer, the precipitates were then resuspended in 0.2 M HCl overnight at 4°C with mild agitation. After centrifugation at 500 g for 10 min, histones in the supernatant were harvested for further analysis. Tris-base was added to the histone fraction for neutralization before SDS-PAGE. Protein gel stained with Coomassie blue was used as the loading control (Beyotime, #P0017F, China).

2.12. Western Blotting

The frozen heart tissues or cultured cells were lysed with ice-cold RIPA lysis buffer supplemented with protease inhibitor cocktail (Roche), PMSF, Na₂VO₃, and deacetylase inhibitor cocktail (Roche). The supernatant was harvested by centrifuging at 13000 g for 15 min at 4°C. The protein was separated by SDS-PAGE and transferred onto the polyvinylidene fluoride (PVDF) membranes for immunoblotting. The PVDF membrane was blocked in 5% nonfat milk and then incubated with primary antibodies overnight at 4°C. The primary antibodies included anti-FOXO3A (10849-1-AP, Proteintech), anti-SOD2 (24127-1-AP, Proteintech), anti-GAPDH (10494-1-AP, Proteintech), anti-histone H3 (ab1791, Abcam), and anti-acetylated histone H3K9 (ab32129, Abcam) antibodies. The signal intensities were visualized by the ECL Western blotting Detection kit (#P10100, ECM) after incubation with HRP-conjugated secondary antibodies (#SA00001-1 and #SA00001-2; Proteintech) and quantified by the ImageJ software (National Institutes of Health, Bethesda, MD, USA).

2.13. Chromatin Immunoprecipitation (ChIP) Analysis

ChIP was performed using the High Sensitivity ChIP Assay Kit (Zoektech#A01-0325, China). According to the manufacturer’s protocol, the protein-DNA complex was cross-linked with formaldehyde, sonicated, and immunoprecipitated with antibody-conjugated protein A/G agarose beads (Santa Cruz Biotechnology, Santa Cruz, CA) at 4°C overnight. The antibodies used for ChIP were normal mouse IgG (Santa Cruz Biotechnology), anti-histone H3 (ab1791, Abcam), and anti-acetylated histone H3K9 (ab32129, Abcam). The immunoprecipitated DNA was recovered with proteinase K and purified with phenol/chloroform precipitation. The precipitated DNA was analyzed with SYBR green qPCR. As for the H3K9 promoter binding assay, the primer sets used as follows:

FOXO3A-0.4 K-F,GGTTTTCTTGCAGTCCGAGAG;

FOXO3A-0.4 K-R,GACCCGCTAAGAAGATCTGAGG;

FOXO3A-0.6 K-F,GGGTCGGTCCTCTCTCGTT;

FOXO3A-0.6 K-R,GCAACTCCCGTCTTTTCCTC;

FOXO3A-1 k-F,TCCCCAGGTCTATCCGTTCT;

FOXO3A-1 K-R,GGGCTCTTGCTCTCTCCTCT;

FOXO3A-1.2 K-F,AACTCTCTCTTCGCGCTTCC;

FOXO3A-1.2 K-R,TTGGGCTCTTGCTCTCTCCT;

MT2-0.1 K-F,AGAGCAGGACGGACTTTTG;

MT2-0.1 K-R,CGAGCCATTATCTCAAGGACT;

MT2-0.2 K-F,GGGTACTACTGGCTGCTCCT;

MT2-0.2 K-R,CAAAGAACTCGGGTGCAAG.

2.13.1. Statistical Analysis

GraphPad Prism v.9.0.1 (GraphPad, La Jolla, CA) was employed for statistical analysis. The Shapiro-Wilk normality test was performed to determine the data distribution. All data were normally distributed and presented as the deviation (SD). Paired or unpaired two-tailed Student’s -tests were selected to compare two groups. One-way analysis of variance (ANOVA), followed by Tukey’s multiple comparisons test, was performed to determine the differences . was considered to be statistically significant.

3. Results

3.1. Ketone Bodies Protected the Hearts against LPS-Induced Acute Myocardial Injury and Cardiac Dysfunction

Male C57BL/6 J mice were exposed to LPS (20 mg/kg, i.p.) to induce septic cardiomyopathy, as described previously [5, 8]. In the KE pretreatment group, an almost two-fold increase was detected in the levels of circulating ketone bodies, especially that of β-OHB (Figure 1(a)). Remarkably, the levels of total ketone bodies and their two primary forms, namely, β-OHB and AcAc, increased in the heart tissues (Figure 1(b)), which indicated that KE gavage significantly enhanced the levels of ketone bodies both in the bloodstream and in the heart tissues (Figures 1(a) and 1(b)).

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Figure 1

Ketone bodies protected the hearts against LPS-induced acute myocardial injury and cardiac dysfunction. (a). Blood β-OHB levels in Con, LPS, and mice ( per group). (b). The levels of ketone bodies (β-OHB; AcAc) in the Con, LPS, and hearts ( per group). (c). Representative echocardiography images of the Con, LPS, and hearts ( per group). (d–f) Cardiac function was indicated by ejection fractions (EF) (d), shortening fraction (FS) (e), and cardiac output (CO) (f) ( per group). (g and h) The levels of CK-MB (g) and LDH (h) in the plasma samples ( per group). (i) Representative images of hematoxylin and eosin- (H&E-) stained left ventricle tissue sections ( per group). Scale μm. Con, Control; LPS, lipopolysaccharide; and KE, ketone ester. Data are presented as the . Statistical comparisons were conducted by one-way ANOVA, followed by Tukey’s multiple comparisons test (a, b, d, e, f, g, and h). The exact values were reported for the indicated comparisons, and was considered statistically significant. , , , and for the indicated comparisons. ns: no significant difference.

Six hours after LPS injection, echocardiography revealed that the LPS-treated mice demonstrated a sharp decrease in LVEF, FS, and CO (Figures 1(c)–1(f)), which established that LPS-induced acute septic cardiomyopathy. Consistently, the plasma levels of cardiac damage markers, CK-MB and LDH (Figures 1(g) and 1(h)) were substantially higher in the LPS-treated mice compared with the control group. These results suggested that LPS-induced myocardial injury and reduced cardiac function. Compared with the LPS group, the mice in the group appeared to have increased LVEF, FS, and CO (Figures 1(c)–1(f)) and decreased levels of cardiac damage markers (Figures 1(g) and 1(h)), which implied that the ketone bodies mitigated heart injury and preserved heart contractile function (Figures 1(c)–1(h)).

Furthermore, H&E staining indicated that the myocardial cells were sparse and disordered, with interstitial edema and abundant inflammatory cell infiltration in the LPS group compared with the control group (Figure 1(i)). Interestingly, KE treatment ameliorated the structural disorderliness in the heart of LPS-treated mice, which meant that the cardiomyocytes were more organized and have fewer inflammatory cell infiltrates and granulocytic aggregates (Figure 1(i)). These results suggest that the ketone bodies prevented LPS-induced septic myocardial injury and cardiac dysfunction.

3.2. Ketone Bodies Mitigated Cardiac Mitochondrial Dysfunction and Oxidative Stress in Septic Cardiomyopathy

Mitochondrial abnormalities are closely related to cardiac dysfunction [15, 32]. To visualize the ultrastructural alterations of the mitochondrion in the hearts of LPS-treated mice, we conducted transmission electron microscopic analyses. The hearts of LPS-treated mice showed notable cytoarchitectural destruction, especially disrupted mitochondria, as shown with mitochondrial swelling along with the formation of internal vesicles, disorganized cristae, and lowered matrix density (Figure 2(a)). Intriguingly, pretreatment with ketone ester preserved the heart mitochondrial ultrastructure to some extent (Figure 2(a)). It is well known that the disruption of mitochondrial morphological structure and functional dysregulation often occur simultaneously. Correspondingly, seahorse analysis confirmed that LPS induced an apparent decrease in pyruvate/malate-supported mitochondrial respiratory function (Figures 2(b)–2(d)), while ketone bodies improved both the ADP-stimulated basal OCR and FCCP-stimulated maximal OCR (Figures 2(b)–2(d)).

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Figure 2

Ketone bodies mitigated cardiac mitochondrial dysfunction and oxidative stress in septic cardiomyopathy. (a) Representative transmission electron microscopy images of the Con, LPS, and heart sections ( per group). Scale . (b–d) The oxygen consumption rate (OCR) curve in the presence of pyruvate and malate of the isolated mitochondria from the mouse hearts (b). The ADP-stimulated OCR (c) and FCCP-stimulated OCR (d) ( per group). (e) Representative images of dihydroethidium (DHE) staining in Con, LPS, and hearts ( fields, from 3 hearts per group). Scale μm or 50 μm. (f and g) Western blotting of 2,4-dinitrophenylhydrazone (DNP) in the heart tissues from Con, LPS, and mice (f) ( per group). The protein levels of DNP were normalized to the GAPDH levels, and the data were expressed as the fold change relative to the control (g) (n =5 per group). (h) Malondialdehyde (MDA) levels in the heart tissues ( per group). (i) Superoxide dismutase (SOD) activity in the heart tissues ( per group). Con: Control; LPS: lipopolysaccharide; KE: ketone ester; ADP: adenosine diphosphate; Oligo: oligomycin A; FCCP: trifluorocarbonyl cyanide phenylhydrazone; and AA: antimycin A. Data are presented as the . Statistical comparisons were conducted using one-way ANOVA, followed by Tukey’s multiple comparisons test (c, d, g, h, and i). The exact values were reported for the indicated comparisons, with considered statistical significance. , , , and for the indicated comparisons.

The mitochondrion is the primary source of intracellular ROS and is extremely susceptible to oxidative stress. Therefore, we investigated whether the benefit offered by the ketone bodies was mediated by suppressing oxidative stress. The fluorescence intensity of DHE-stained cardiac tissue increased in the LPS group, which suggested a high level of ROS production (Figure 2(e)). Moreover, excessive protein carbonylation, an irreversible oxidative protein modification (Figures 2(f) and 2(g)), increased level of MDA, and decreased SOD activity were observed in the hearts of LPS-treated mice (Figures 2(h) and 2(i)). Notably, the hearts showed reduced fluorescence intensity of DHE, accompanied by mitigated protein carbonylation, lowered MDA level, and enhanced SOD activity (Figures 2(e)–2(i)). These results suggest that while LPS-induced septic heart injury was associated with oxidative stress damage, ketone bodies mitigated cardiac oxidative stress, and improved mitochondrial function in septic cardiomyopathy.

3.3. β-OHB Alleviated Oxidative Stress and Enhanced Aerobic Respiration in H9C2 Cells Exposed to MCM

An excessive inflammatory response has been acknowledged as the hallmark of septic cardiomyopathy [3, 9]. In sepsis, inflammatory infiltration caused by macrophages secreting several cytokines is the leading cause of myocardial injury [3, 4]. To verify the effect of ketone bodies on myocardial mitochondrial oxidative stress, H9C2 cells were incubated with LPS-stimulated MCM to mimic the pathological process of septic cardiomyopathy and were treated with β-OHB for 24 h (Figure 3(a)). ELISA proved that the levels of inflammatory cytokines, including IL-1β, IL-6, and TNF-α, were drastically elevated in the MCM-cultured cells (Figure 3(b)).

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Figure 3

β-OHB alleviated oxidative stress and enhanced aerobic respiration in H9C2 cells exposed to MCM. (a) Schematic representation of the experimental protocol. (b) The levels of inflammatory cytokines in LPS-stimulated macrophage conditioned medium (MCM) () and standard cell culture medium (DMEM, Med) with 10% fetal calf serum. (c). Representative fluorescent images of H9C2 cells stained with MitoSOX red after the indicated treatments. Scale μm. The nuclei were visualized with Hoechst staining. Scale μm. (d). The fluorescence intensity of MitoSOX-stained H9C2 cells after the indicated treatments ( per group). (e and f) The oxygen consumption rate (OCR) curve in the presence of pyruvate and L-glutamine in H9C2 cells after the indicated treatments (e) and the basal respiration and spare respiratory capacity (OCR_FCCP–OCR_basal) (f) (–6 per group). Oligo: Oligomycin A; A A./Rot: antimycin A and rotenone. Data are presented as the . Statistical comparisons were conducted by one-way ANOVA, followed by Tukey’s multiple comparisons test (b, d, and f). The exact values are reported for the indicated comparisons, and indicates statistical significance. and for the indicated comparisons.

Moreover, the intensity of MitoSOX fluorescence, an indicator of mitochondrial superoxide, was remarkably enhanced in the MCM-cultured H9C2 cells. Meanwhile, β-OHB treatment mitigated ROS production (Figures 3(c) and 3(d)). Additionally, seahorse analysis showed that the mitochondrial respiratory function of H9C2 cells was also improved by β-OHB, indicated with both basal respiration and spare respiratory capacity (Figures 3(e) and 3(f)). Intriguingly, the additive effect of β-OHB was not observed, and the nonspecific ROS scavenger N-acetylcysteine (NAC) in the H9C2 cells exposed to MCM suggested that β-OHB exhibited antioxidant effects similar to those of NAC on cellular aerobic respiration (Figures 3(e) and 3(f)). Together, these data imply the protective effect of β-OHB as an antioxidant on myocardial oxidative stress and mitochondrial function.

3.4. β-OHB Alleviated Oxidative Stress and Improved Mitochondrial Function via HDAC Inhibition in MCM-Cultured H9C2 Cells

As an endogenous and specific inhibitor of HDAC, β-OHB has been reported to confer significant resistance against oxidative stress [23] (Figure 4(a)). To identify whether the protective effect of β-OHB on mitochondrial function and oxidative stress was mediated by histone acetylation in septic cardiomyopathy, ITSA1, an activator of histone deacetylase, or entinostat, an inhibitor of HDAC was used to regulate histone acetylation in MCM-cultured H9C2 cells. It is worth noting that the suppression of mitochondrial superoxide by β-OHB could be abolished by ITSA1 or mimicked by entinostat (Figures 4(b)–4(d)), which indicated that β-OHB inhibited mitochondrial ROS production in response to histone acetylation status (Figures 4(b)–4(d)).

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Figure 4

β-OHB alleviated oxidative stress and improved mitochondrial function via HDAC inhibition in MCM-treated H9C2 cells. (a) ITSA1 (HDAC activator) and entinostat (HDAC inhibitor) were used in this study. (b) Representative fluorescent images of H9C2 cells stained with MitoSOX red to assess the mitochondrial ROS generation after the indicated treatments ( per group). Scale μm. The nuclei were visualized with Hoechst staining. Scale μm. (c). The fluorescence intensity of MitoSOX-stained H9C2 cells after the indicated treatments ( per group). (d). Representative MitoSOX flow cytometry analysis in H9C2 cells after the indicated treatments ( per group). (e and f) The oxygen consumption rate (OCR) curve in the presence of pyruvate and L-glutamine in H9C2 cells after the indicated treatments (e), and the basal respiration and spare respiratory capacity (OCR_FCCP−OCR_basal) (f) ( per group). Oligo: Oligomycin A; A.A./Rot: antimycin A and rotenone. Data are presented as the . Statistical comparisons were conducted by one-way ANOVA, followed by Tukey’s multiple comparisons test (c and f). The exact values are reported for the indicated comparisons, and indicates statistical significance. and for the indicated comparisons.

As expected, seahorse analysis showed that the improvement of cellular aerobic respiration in MCM-cultured H9C2 cells by β-OHB was similar to that of entinostat but opposite to that of ITSA1 (Figures 4(e) and 4(f)), thereby signifying that β-OHB improved mitochondrial function. Collectively, these results demonstrated that β-OHB protected the mitochondria against oxidative stress damage and improved mitochondrial function via HDAC inhibition in MCM-cultured H9C2 cells.

3.5. Ketone Bodies Enhanced FoxO3a And MT2 Expressions by Promoting Histone H3 Lysine 9 Acetylation

HDAC and histone acetyltransferase (HAT) are responsible for reversible changes in the histone acetylation status. Inhibition of HDAC by β-OHB was correlated with global changes in transcription, including genes encoding of the oxidative stress resistance factors, FoxO3a, and MT2 [23, 33, 34] (Figure 5(a)). The mRNA levels of FoxO3a and MT2 were estimated in the H9C2 cells. Remarkably, the expressions of FoxO3a and MT2 mRNA were significantly decreased in MCM-cultured H9C2 cells, while both were elevated after treatment with 5 mM β-OHB (Figures 5(b) and 5(c)). To comprehend the biological impact of β-OHB on antioxidant genes, β-OHB was used, in combination with the HDAC activator ITSA1 or the inhibitor entinostat, to detect the expressions of FoxO3a and MT2. ITSA1 blocked the upregulated expressions of FoxO3a and MT2 induced by β-OHB (Figures 5(b) and 5(c)). In contrast, entinostat did not alter the effect of β-OHB on the expressions of these genes (Figure 5(b) and 5(C)), which confirmed that β-OHB offered resistance against oxidative stress via HDAC inhibition.

(a)

(b)

(c)

(d)

(e)

(f)

(g)

(h)

(i)

(j)

(k)

(l)

Figure 5

The ketone bodies enhanced FoxO3a and MT2 expression by promoting histone H3 lysine 9 acetylation. (a) HDAC exerts oxidative stress resistance through the FoxO3a/MT2 pathway. FoxO3a: Forkhead box O3; MT2: Metallothionein 2A. (b and c) qRT-PCR analysis of FoxOa3 (b) and MT2 (c) in H9C2 cells after the indicated treatments (–8 per group). (d and e) Western blotting of the acetylation of H3K9 in purified histones from H9C2 cells after the indicated treatments (d). The quantification of the band intensity (e). Acetylation is normalized to the total histone content H3 and reported to be relative to the MCM-exposed cells. Coomassie blue staining was used as the gel loading control (–6 per group). (f) Chromatin from H9C2 cells after the indicated treatments were immunoprecipitated with anti-histone H3 or anti-AcH3K9, and the purified DNA was analyzed with primer pairs specific for the FoxO3a or MT2 promoters. The results are shown as the ratios of AcH3K9 to total histone H3 (–6 per group). (g–i) Western blotting of FoxO3a and SOD2 in H9C2 cells after the indicated treatments (g). Quantification of the band intensity (h and i). The protein levels of FoxO3a and SOD2 were normalized to those of GAPDH, and the data are expressed as fold changes relative to the control value (–9 per group). (j–l) Western blotting of FoxO3a and SOD2 in the heart tissues from control, LPS, and mice (j). Quantification of the band intensity (k and l). The protein levels of FoxO3a and SOD2 were normalized to those of the GAPDH, and the data are expressed as the fold change relative to the control value ( per group). Data are presented as the . Statistical comparisons were conducted using one-way ANOVA, followed by Tukey’s multiple comparisons test (b, c, d, e, f, h, i, k, and l). The exact values are reported for the indicated comparisons, and indicates statistical significance. , , and for the indicated comparisons.

Accumulating evidence suggests that histone acetylation promotes the binding of FoxO3a and MT2 to their promoters and enhances their expression [23, 33]. AcH3_K9 has been identified to play a crucial role in activating gene expression [35, 36]. Correspondingly, Western blot analysis of AcH3_k9 in the purified histone showed that β-OHB triggered histone acetylation in MCM-cultured H9C2 cells (Figures 5(d) and 5(e)). Furthermore, ChIP analysis of the Foxo3a and MT2 promoters with several distinct primer pairs revealed increased AcH3_K9 binding to these gene promoters under high β-OHB exposure (Figure 5(f)), which confirmed the role of β-OHB in epigenetics.

Subsequently, the protein expressions of FoxO3a and the downstream target SOD2, which contributes to antioxidative protection, were upregulated by β-OHB in MCM-cultured H9C2 cells, having the same effect as that of an AcH3_K9-induced active promoter (Figures 5(g)–5(i)). As expected, ITSA1 abrogated the promoting effects of β-OHB on protein expression, whereas entinostat exerted the same effect as β-OHB (Figures 5(g)–5(i)). Furthermore, elevated expressions of FoxO3A and SOD2 were found in septic hearts, thereby, supporting the in vitro findings (Figures 5(j)–5(l)).

Collectively, these data suggested that β-OHB acts as an HDAC inhibitor, which enhances histone acetylation, to activate the antioxidant FoxO3a/MT2 pathway, thereby preventing ROS production and offering mitochondrial protection in septic cardiomyopathy.

4. Discussion

In this study, the ketone body β-OHB was shown to prevent LPS-induced myocardial injury and cardiac dysfunction. Mechanistically, as an HDAC inhibitor, β-OHB activated the antioxidant FoxO3a/MT2 pathway. This response enhanced redox homeostasis and improved mitochondrial function (Figure 6). These findings, therefore, suggest that β-OHB is an effective agent for myocardial protection in sepsis.

During sepsis, a sharp decrease in the contractile function of the heart and severe myocardial damage were observed. Fortunately, the disruption of structure and the disorder of function in the septic hearts could be prevented by KE preconditioning. In the normal physiological conditions, the cardiac contractive function is highly energy consuming and depends much on mitochondrial OXPHOS for ATP generation [37, 38]. Well-organized cristae and large mitochondrial matrices are indispensable for supercomplex formation and are closely associated with electron transfer efficiency [39, 40]. In line with previous studies [9, 15], disrupted mitochondrial ultrastructure and depressed mitochondrial OXPHOS were observed in the hearts of LPS-treated mice. The preconditioning of KE contributed to high levels of β-OHB, which ameliorated the damage to the mitochondrial ultrastructure of the myocardium. Furthermore, β-OHB improved pyruvate/malate-supported mitochondrial respiration, which rescued ATP production in the septic hearts. In addition, β-OHB reduced global carbonylation proteins and lipid oxidation levels and increased SOD2 activity, indicating that β-OHB prevents ROS overproduction for mitochondrial protection. Therefore, this study provides direct evidence to support that β-OHB exerts a protective effect in septic cardiomyopathy and that the primary regulatory machinery fine-tunes mitochondrial performance and ameliorates oxidative stress.

Ketone bodies are essential energy sources for life activities, and β-OHB accounts for approximately 70% of the total circulating ketones [21]. The level of β-OHB in the bloodstream increases to 1–2 mM or even higher (6–8 mM) during prolonged fasting, while the concentration could be increased to >25 mM in diabetic ketoacidosis [18, 21]. Intravenously administered β-OHB could rapidly increase the β-OHB concentrations to >2 mmol/L without exerting any deleterious side effects, ascertaining the potential benefit of β-OHB in specific disease states, such as stroke or traumatic brain injury [41]. In chronic heart failure, myocardial ischemia and diabetic cardiomyopathy, as an energy source, β-OHB can exert beneficial effects to meet myocardial oxygen demand [20, 42]. β-OHB restored doxorubicin-induced left ventricular dysfunction and prevented cardiac remodeling through sustaining mitochondrial membrane potential integrity [43]. However, most studies have focused on the effects of β-OHB in case of long-term exposure [44]. In contrast, septic cardiomyopathy is an acute cardiac injury characterized by a sudden decline in LVEF in 20% of patients in the first 6 h of septic shock [3]. Overtime, the release of inflammatory factors attacks the myocardial mitochondria and results in ROS outbreak [45]. Therefore, in this study, the biochemical advantages of acute ketosis in septic cardiomyopathy were explored using short-term KE supplements. Interestingly, the ingestion of KE by LPS-challenged mice for 3 days and the exposure of MCM-cultured H9C2 cells to high concentrations of β-OHB resulted in reduced ROS production. Our results demonstrated that β-OHB is an effective and practical treatment for improving myocardial mitochondrial performance in septic cardiomyopathy.

In addition to serving as alternative biofuel for extrahepatic tissues, for example, the heart, brain, and skeletal muscle, ketone bodies have also been shown to play pivotal roles in signal transduction, protein post-translational modification, and inflammation regulation [23, 46]. In recent years, β-OHB has been shown to be a novel HDAC inhibitor owing to its structural similarity with butyrate (a traditional HDAC inhibitor) [23]. AcH3_K9 is crucial and linked to the active promoter [36]. Hence, the histone acetylation levels of AcH3_K9 were measured, and β-OHB was found to trigger histone acetylation, which is consistent with the results of a previous experiment on human embryonic kidney cells (HEK293) [23]. The role of AcH3_K9-activated transcription factor FoxO3a has been associated with antioxidant stress in various organisms [47]. In our study, ChIP analysis of the FoxO3a and MT2 promoters revealed increased AcH3_K9 due to high β-OHB exposure. The FoxO3a and MT2 genes, which encode antioxidant proteins, for example, SOD and catalase dismutase, are activated when histone acetylation increases [14, 48]. At the protein level, β-OHB was noted to enhance the expressions of FoxO3a and SOD2 in septic hearts. Manabu Nagao et al. reported that the accumulation of β-OHB in the failing hearts occurs as a compensatory response to oxidative stress [49]. Both these studies reported an antioxidative effect of β-OHB in the stressed hearts; however, the key findings of the two studies were different. The Nagao paper suggested that the endogenous accumulated β-OHB in response to pressure overload or H₂O₂ exposure could protect cardiomyocytes, while our study demostrated the therapeutic effects of β-OHB supplementation on LPS-induced septic cardiomyopathy. Importantly, we provided new mechanistic insights by which β-OHB alleviated oxidative stress and improved the mitochondrial function in septic hearts (inhibition of HDAC by β-OHB to promote H3K9 acetylation). Above all, our findings demonstrated that β-OHB, an endogenous HDAC inhibitor, mediates antioxidant gene expression, and integrates redox homeostasis with epigenetic alterations. This finding adds a new mechanism to the reported function of β-OHB as a signaling molecule in septic cardiomyopathy.

Our study has several strengths. We pioneered the use of ketone bodies as a pharmacologic approach to prevent systolic myocardial dysfunction and rescue poor heart pumping ability in septic cardiomyopathy, thereby providing a basis for clinical therapy. Subsequently, state-of-the-art techniques, such as seahorse mitochondrial analysis and ChIP analysis, were exploited to uncover the role of β-OHB in signal translation and protein modification. However, we acknowledge that there are several limitations in the present study. First, the critical impacts of β-OHB on antioxidants in septic cardiomyopathy were not tested in vivo, such as β-OHB dehydrogenase (BDH1)-knockout mice, to verify the outcomes. Second, the effects of prolonged ketone body exposure and the duration of these effects after withdrawal were not investigated in this study. Third, β-OHB-initiated cardiac effects exhibit sex differences [5, 26]. Hence, caution should be exercised while extrapolating our findings to females and other mouse strains.

5. Conclusions

Our study has demonstrated that ketone bodies, especially β-OHB, activate antioxidant pathways by acting as HDAC inhibitors and improve mitochondrial respiratory function, thus offering functional cardiac protection in septic cardiomyopathy. These promising findings suggest the possibility of applying ketone bodies for the clinical treatment of septic heart injury.

Data Availability

The data that support the findings of this study are available from the corresponding author on reasonable request.

Conflicts of Interest

The authors declare that they have no conflicts of interest.

Authors’ Contributions

Liwei Ji, Qinqin He, and Yinghai Liu contributed to the work equally.

Acknowledgments

This study was supported, in part, by grants from the Key Research and Development Program of Sichuan Province (22ZDYF2138), the National Natural Science Foundation of China (81970715, 81970346, 82170360, 81873500, and 81971806), the Key Research Program of National Clinical Research Center for Geriatrics (Z20191004), the Innovation Spark Project of Sichuan University (2018SCUH0065), and the 1.3.5 Project for Disciplines of Excellence, West China Hospital, Sichuan University (ZYGD18014). Additionally, the authors thank Wei Ou (Department of Anesthesiology, Laboratory of Mitochondria and Metabolism, West China Hospital of Sichuan University) for technical assistance. The authors would like to thank MJEditor (http://www.mjeditor.com) for providing their English editing services during the preparation of this manuscript.

Supplementary Materials

Supplementary file.pdf: the unedited gels for this study. (Supplementary Materials)

References

L. Martin, M. Derwall, S. al Zoubi et al., “The septic heart: current understanding of molecular mechanisms and clinical implications,” Chest, vol. 155, no. 2, pp. 427–437, 2019.
View at: Publisher Site | Google Scholar
C. Fleischmann, A. Scherag, N. K. Adhikari et al., “Assessment of global incidence and mortality of hospital-treated sepsis. Current estimates and limitations,” American Journal of Respiratory and Critical Care Medicine, vol. 193, no. 3, pp. 259–272, 2016.
View at: Publisher Site | Google Scholar
S. M. Hollenberg and M. Singer, “Pathophysiology of sepsis-induced cardiomyopathy,” Nature Reviews Cardiology, vol. 18, no. 6, pp. 424–434, 2021.
View at: Publisher Site | Google Scholar
T. Van Der Poll, F. L. van de Veerdonk, B. P. Scicluna, and M. G. Netea, “The immunopathology of sepsis and potential therapeutic targets,” Nature Reviews Immunology, vol. 17, no. 7, pp. 407–420, 2017.
View at: Publisher Site | Google Scholar
K. Drosatos, R. S. Khan, C. M. Trent et al., “Peroxisome proliferator–activated receptor-γ activation prevents sepsis-related cardiac dysfunction and mortality in mice,” Circulation Heart Failure, vol. 6, no. 3, pp. 550–562, 2013.
View at: Publisher Site | Google Scholar
H. C. Prescott and D. C. Angus, “Enhancing recovery from sepsis: a review,” JAMA, vol. 319, no. 1, pp. 62–75, 2018.
View at: Publisher Site | Google Scholar
W. Wasyluk, P. Nowicka-Stążka, and A. Zwolak, “Heart metabolism in sepsis-induced cardiomyopathy—unusual metabolic dysfunction of the heart,” International Journal of Environmental Research and Public Health, vol. 18, no. 14, p. 7598, 2021.
View at: Publisher Site | Google Scholar
Y. Li, Y. F. Feng, X. T. Liu et al., “Songorine promotes cardiac mitochondrial biogenesis via Nrf2 induction during sepsis,” Redox Biology, vol. 38, article 101771, 2021.
View at: Publisher Site | Google Scholar
K. Mantzarlis, V. Tsolaki, and E. Zakynthinos, “Role of oxidative stress and mitochondrial dysfunction in sepsis and potential therapies,” Oxidative Medicine and Cellular Longevity, vol. 2017, Article ID 5985209, 10 pages, 2017.
View at: Publisher Site | Google Scholar
G. Stanzani, M. R. Duchen, and M. Singer, “The role of mitochondria in sepsis-induced cardiomyopathy,” Biochimica et Biophysica Acta - Molecular Basis of Disease, vol. 1865, no. 4, pp. 759–773, 2019.
View at: Publisher Site | Google Scholar
I. Martinez-Reyes and N. S. Chandel, “Mitochondrial TCA cycle metabolites control physiology and disease,” Nature Communications, vol. 11, no. 1, p. 102, 2020.
View at: Publisher Site | Google Scholar
N. B. Madungwe, N. F. Zilberstein, Y. Feng, and J. C. Bopassa, “Critical role of mitochondrial ROS is dependent on their site of production on the electron transport chain in ischemic heart,” American Journal of Cardiovascular Disease, vol. 6, no. 3, pp. 93–108, 2016.
View at: Google Scholar
H. Sies, “Oxidative stress: a concept in redox biology and medicine,” Redox Biology, vol. 4, pp. 180–183, 2015.
View at: Publisher Site | Google Scholar
H. Sies and D. P. Jones, “Reactive oxygen species (ROS) as pleiotropic physiological signalling agents,” Nature Reviews Molecular Cell Biology, vol. 21, no. 7, pp. 363–383, 2020.
View at: Publisher Site | Google Scholar
J. E. Chipuk, J. N. Mohammed, J. D. Gelles, and Y. Chen, “Mechanistic connections between mitochondrial biology and regulated cell death,” Developmental Cell, vol. 56, no. 9, pp. 1221–1233, 2021.
View at: Publisher Site | Google Scholar
C. Poggi and C. Dani, “Sepsis and oxidative stress in the newborn: from pathogenesis to novel therapeutic targets,” Oxidative Medicine and Cellular Longevity, vol. 2018, Article ID 9390140, 14 pages, 2018.
View at: Publisher Site | Google Scholar
S. Selvaraj, D. P. Kelly, and K. B. Margulies, “Implications of altered ketone metabolism and therapeutic ketosis in heart failure,” Circulation, vol. 141, no. 22, pp. 1800–1812, 2020.
View at: Publisher Site | Google Scholar
Y. Deng, M. Xie, Q. Li et al., “Targeting mitochondria-inflammation circuit by β-Hydroxybutyrate mitigates HFpEF,” Circulation Research, vol. 128, no. 2, pp. 232–245, 2021.
View at: Publisher Site | Google Scholar
Y. H. Youm, K. Y. Nguyen, R. W. Grant et al., “The ketone metabolite β-hydroxybutyrate blocks NLRP3 inflammasome-mediated inflammatory disease,” Nature Medicine, vol. 21, no. 3, pp. 263–269, 2015.
View at: Publisher Site | Google Scholar
Y. Arima, Y. Izumiya, T. Ishida et al., “Myocardial ischemia suppresses ketone body utilization,” Journal of the American College of Cardiology, vol. 73, no. 2, pp. 246-247, 2019.
View at: Publisher Site | Google Scholar
P. Puchalska and P. A. Crawford, “Multi-dimensional roles of ketone bodies in fuel metabolism, signaling, and therapeutics,” Cell Metabolism, vol. 25, no. 2, pp. 262–284, 2017.
View at: Publisher Site | Google Scholar
T. Shimazu, M. D. Hirschey, J. Newman et al., “Suppression of oxidative stress by β-hydroxybutyrate, an endogenous histone deacetylase inhibitor,” Science, vol. 339, no. 6116, pp. 211–214, 2013.
View at: Publisher Site | Google Scholar
G. Hong, D. Zheng, L. Zhang et al., “Administration of nicotinamide riboside prevents oxidative stress and organ injury in sepsis,” Free Radical Biology & Medicine, vol. 123, pp. 125–137, 2018.
View at: Publisher Site | Google Scholar
J. Zhong, Y. Tan, J. Lu et al., “Therapeutic contribution of melatonin to the treatment of septic cardiomyopathy: a novel mechanism linking Ripk3-modified mitochondrial performance and endoplasmic reticulum function,” Redox Biology, vol. 26, article 101287, 2019.
View at: Publisher Site | Google Scholar
D. Kokkinaki, M. Hoffman, C. Kalliora et al., “Chemically synthesized Secoisolariciresinol diglucoside (LGM2605) improves mitochondrial function in cardiac myocytes and alleviates septic cardiomyopathy,” Journal of Molecular and Cellular Cardiology, vol. 127, pp. 232–245, 2019.
View at: Publisher Site | Google Scholar
C. Ari, C. Murdun, C. Goldhagen et al., “Exogenous ketone supplements improved motor performance in preclinical rodent models,” Nutrients, vol. 12, no. 8, p. 2459, 2020.
View at: Publisher Site | Google Scholar
P. J. Cox, T. Kirk, T. Ashmore et al., “Nutritional ketosis alters fuel preference and thereby endurance performance in athletes,” Cell Metabolism, vol. 24, no. 2, pp. 256–268, 2016.
View at: Publisher Site | Google Scholar
L. Suissa, P. Kotchetkov, J. M. Guigonis et al., “Ingested ketone ester leads to a rapid rise of acetyl-CoA and competes with glucose metabolism in the brain of non-fasted mice,” International Journal of Molecular Sciences, vol. 22, no. 2, p. 524, 2021.
View at: Publisher Site | Google Scholar
X. Gu, Y. Ma, Y. Liu, and Q. Wan, “Measurement of mitochondrial respiration in adherent cells by seahorse XF96 cell Mito stress test,” STAR Protocols, vol. 2, no. 1, article 100245, 2021.
View at: Publisher Site | Google Scholar
W. Ou, Y. Liang, Y. Qing et al., “Hypoxic acclimation improves cardiac redox homeostasis and protects heart against ischemia-reperfusion injury through upregulation of O-GlcNAcylation,” Redox Biology, vol. 43, p. 101994, 2021.
View at: Publisher Site | Google Scholar
A. A. Kumar, D. P. Kelly, and J. A. Chirinos, “Mitochondrial dysfunction in heart failure with preserved ejection fraction,” Circulation, vol. 139, no. 11, pp. 1435–1450, 2019.
View at: Publisher Site | Google Scholar
Y. Liu, X. Ao, W. Ding et al., “Critical role of FOXO3a in carcinogenesis,” Molecular Cancer, vol. 17, no. 1, p. 104, 2018.
View at: Publisher Site | Google Scholar
S. Martire, A. A. Gogate, A. Whitmill et al., “Phosphorylation of histone H3.3 at serine 31 promotes p300 activity and enhancer acetylation,” Nature Genetics, vol. 51, no. 6, pp. 941–946, 2019.
View at: Publisher Site | Google Scholar
G. S. Shadel and T. L. Horvath, “Mitochondrial ROS signaling in organismal homeostasis,” Cell, vol. 163, no. 3, pp. 560–569, 2015.
View at: Publisher Site | Google Scholar
P. H. Willems, R. Rossignol, C. E. Dieteren, M. P. Murphy, and W. J. H. Koopman, “Redox homeostasis and mitochondrial dynamics,” Cell Metabolism, vol. 22, no. 2, pp. 207–218, 2015.
View at: Publisher Site | Google Scholar
D. Milenkovic, J. N. Blaza, N. G. Larsson, and J. Hirst, “The enigma of the respiratory chain supercomplex,” Cell Metabolism, vol. 25, no. 4, pp. 765–776, 2017.
View at: Publisher Site | Google Scholar
S. Cogliati, C. Frezza, M. E. Soriano et al., “Mitochondrial cristae shape determines respiratory chain supercomplexes assembly and respiratory efficiency,” Cell, vol. 155, no. 1, pp. 160–171, 2013.
View at: Publisher Site | Google Scholar
H. White, A. J. Heffernan, S. Worrall, and M. Thomas, “A systematic review of intravenous β-hydroxybutyrate use in humans - a promising future therapy?” Frontiers in Medicine, vol. 8, article 740374, 2021.
View at: Publisher Site | Google Scholar
R. Pietschner, J. Kolwelter, A. Bosch et al., “Effect of empagliflozin on ketone bodies in patients with stable chronic heart failure,” Cardiovascular Diabetology, vol. 20, no. 1, p. 219, 2021.
View at: Publisher Site | Google Scholar
Y. Liu, X. Wei, M. Wu, B. Xu, and L. Kang, “Cardioprotective roles of β-hydroxybutyrate against doxorubicin induced cardiotoxicity,” Frontiers in Pharmacology, vol. 11, article 603596, 2020.
View at: Publisher Site | Google Scholar
R. Acar, I. Erturk, G. Taskin et al., “Association between eta-Hydroxybutyrate Levels and Survival in Sepsis Patients,” Eurasian Journal of Medical Investigation, vol. 5, no. 1, pp. 39–44, 2021.
View at: Publisher Site | Google Scholar
N. L. Stanski and H. R. Wong, “Prognostic and predictive enrichment in sepsis,” Nature Reviews Nephrology, vol. 16, no. 1, pp. 20–31, 2020.
View at: Publisher Site | Google Scholar
G. Kong, Z. Huang, W. Ji et al., “The ketone metabolite β-Hydroxybutyrate attenuates oxidative stress in spinal cord injury by suppression of class I histone deacetylases,” Journal of Neurotrauma, vol. 34, no. 18, pp. 2645–2655, 2017.
View at: Publisher Site | Google Scholar
J. B. Baell, D. J. Leaver, S. J. Hermans et al., “Inhibitors of histone acetyltransferases KAT6A/B induce senescence and arrest tumour growth,” Nature, vol. 560, no. 7717, pp. 253–257, 2018.
View at: Publisher Site | Google Scholar
K. J. Menzies, H. Zhang, E. Katsyuba, and J. Auwerx, “Protein acetylation in metabolism -- metabolites and cofactors,” Nature Reviews Endocrinology, vol. 12, no. 1, pp. 43–60, 2016.
View at: Publisher Site | Google Scholar
S. Bhattacharya, “Reactive oxygen species and cellular defense system,” Free Radicals in Human Health and Disease, Springer, New Delhi, pp. 17–29, 2015.
View at: Publisher Site | Google Scholar
M. Nagao, R. Toh, Y. Irino et al., “β-Hydroxybutyrate elevation as a compensatory response against oxidative stress in cardiomyocytes,” Biochemical and Biophysical Research Communications, vol. 475, no. 4, pp. 322–328, 2016.
View at: Publisher Site | Google Scholar

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Copyright © 2022 Liwei Ji 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.

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