Abstract
Chronic intrauterine hypoxia is a significant pregnancy complication impacting fetal heart growth, metabolism, and mitochondrial function, contributing to cardiovascular programming of the offspring. PGC1α (peroxisome proliferator-activated receptor γ co-activator 1α) is the master regulator of mitochondrial biogenesis. We investigated the effects of hypoxia on PGC1α expression following exposure at different gestational ages. Time-mated pregnant guinea pigs were exposed to normoxia (NMX, 21% O2) or hypoxia (HPX, 10.5% O2) at either 25-day (early-onset) or 50-day (late-onset) gestation, and all fetuses were extracted at term (term = ~65-day gestation). Expression of nuclear PGC1α, sirtuin 1 (SIRT1), AMP-activated protein kinase (AMPK), and mitochondrial sirtuin 3 (SIRT3) was measured, along with SIRT3 activity and mitochondrial acetylation of heart ventricles of male and female fetuses. Early-onset hypoxia increased (P<0.05) fetal cardiac nuclear PGC1α and had no effect on mitochondrial acetylation of either growth-restricted males or females. Late-onset hypoxia had either no effect or decreased (P<0.05) PCC1α expression in males and females, respectively, but increased (P<0.05) mitochondrial acetylation in both sexes. Hypoxia had variable effects on expression of SIRT1, AMPK, SIRT3, and SIRT3 activity depending on the sex. The capacity of the fetal heart to respond to hypoxia differs depending on the gestational age of exposure and sex of the fetus. Further, the effects of late-onset hypoxia on fetal heart function impose a greater risk to male than female fetuses, which has implications toward cardiovascular programming effects of the offspring.
Similar content being viewed by others
Avoid common mistakes on your manuscript.
Introduction
Chronic intrauterine hypoxia is one of the most significant complications of pregnancy, altering normal placenta and fetal development and leading to fetal growth restriction [1, 2]. Tissue hypoxia disrupts cellular energy metabolism and mitochondrial dysfunction, both of which are at the core of generating oxidative stress and fetal organ dysfunction. Chronic hypoxia generates oxidative stress via electron leak along the respiratory chain, thereby reducing the efficiency of oxidative phosphorylation and altering mitochondrial function [3, 4].
The mitochondria are important cellular organelles for generating energy supply. In early gestation, the fetal heart is reliant on anaerobic glycolysis for ATP [5]. With maturation, the fetal heart increases its capacity for oxidative phosphorylation as it increases its mitochondrial density, ultrastructural organization [6], and cellular compartmentation of metabolic processes [5, 7, 8]. This assures an efficient energy transfer to contractile proteins in accordance with an increasing metabolic demand at the time of birth [5]. Chronic hypoxia disrupts mechanisms associated with both contractile [9, 10] and mitochondrial function in the fetal heart [11,12,13,14]. This has long-term consequences associated with cardiovascular programming of the offspring [15,16,17,18]. Thus, understanding how hypoxia alters mitochondrial function of the fetal heart is important for identifying the underlying mechanisms that initiate developmental programming of cardiovascular disease.
Peroxisome proliferator-activated receptor γ co-activator 1α (PGC1α) is the master regulator of mitochondrial biogenesis via regulation of both nuclear- and mitochondrial-encoded protein expression in several tissues including the heart [19,20,21]. Translocation of PGC1α into the nucleus is regulated by deacetylation by sirtuin 1 (SIRT1) and phosphorylation by AMP-activated protein kinase (AMPK) in the cytosol. While AMPK is a sensor of metabolic conditions, effects of both AMPK and SIRT1 on PGC1α transcription are mediated within the nucleus [19, 22]. Activated-nuclear PGC1α induces expression of transcription factors, such as NRF 1/2 and mitochondrial TFAM, which are transported to the mitochondrial DNA and regulate respiratory complex subunit and SIRT3 expression [19]. SIRT3 is the most important mitochondrial deacetylase, which regulates protein acetylation by acetyl Co A of respiratory complex subunits [23]. The link between PGC1α and nuclear-encoded SIRT3 is important in the regulation of mitochondrial protein acetylation and function [19].
We have previously reported that chronic intrauterine hypoxia disrupts the expression of mitochondrial respiratory complex subunits (CI, CIII, and CV) and alters CI and CIV activities in both left cardiac ventricles and isolated cardiomyocytes of fetal guinea pig hearts [11, 13]. Further, there is a sexual dimorphism in mitochondrial responses of fetal hearts to intrauterine hypoxia, depending on the gestational age of exposure (early vs late gestation) [13]. For example, exposure to hypoxia in early gestation (40–50 days, 65 days = term) increases the expression of mitochondrial CI, CIII, and CV subunits in male fetal heart ventricles, whereas exposure in late gestation decreases the expression of the same subunits in both male and female hearts [13]. These studies show that gestational timing of hypoxia can differentially affect mitochondrial protein expression and, potentially, impact cardiac mitochondrial function.
In adult heart, the importance of PGC1α in the regulation of mitochondrial biogenesis is well established [19,20,21]. Yet, its role in the fetal heart and the effects of gestational hypoxia on PGC1α expression has not been investigated. Given the differential effects of hypoxia on mitochondrial respiratory complex subunit expression shown in our previous study [13], our aim in this study was to determine the effects of hypoxia on upstream signaling of PGC1α as a mechanism of downstream mitochondrial protein activity in fetal hearts. We hypothesized that the hypoxia-induced increase in respiratory complex I, III, and V subunit expression would be mediated by increased PGC1α expression in early-onset hypoxia and decreased with late-onset hypoxia. We further aimed to determine sex differences in this signaling response to assess the fetuses’ vulnerability to the hypoxic challenges.
Methods
All animal procedures using guinea pigs were approved by the University of Maryland Institutional Animal Care and Use Committee in accordance with AAALAC International accreditation (Animal Welfare Assurance no. A3200-01).
Animal Model
Timed-mated pregnant guinea pigs were housed under conditions of either normoxia (room air, NMX) or chronic hypoxia (10.5% O2, HPX) in a normobaric plexiglass chamber, generating maternal [11] and fetal hypoxia, the latter evidenced by fetal cardiac HIF (hypoxia-inducible factor) signaling [24] and oxidative stress [25]. Oxygen levels were reduced in the chamber with N2 gas mixed with room air, monitored with an O2 sensing probe (Reming Bioinstruments, Redfield, NY) and a servo-controlled feedback regulator to maintain a stable 10.5% O2 level. Excess CO2 and H2O vapor were removed by exposing the air mixture to soda lime and silica gel, respectively, Animals were kept in individual box containers within the chamber so food and water, provided ad libitum, could be monitored and replenished every other day. All animals are housed in a temperature-controlled room with a light/dark cycle every 12 h. Similar to our previous study [13], animals were exposed to hypoxia at either 25-day or 50-day gestation (term = ~65-day gestation), corresponding to a duration of 39 and 14d, respectively. Exposure at 25-day gestation corresponds to early stages of trophoblast invasion (~21-day gestation and placental development) in the guinea pig, and exposure at 50-day gestation corresponds to the rapid fetal growth phase, post organogenesis, and placenta maturation [26]. At near term, pregnant guinea pigs were anesthetized (ketamine, 80mg/kg, s.c.; xylazine, 6mg/kg, s.c.) and fetuses extracted via an abdominal incision and uterotomy following subcutaneous administration of 2% lidocaine. Anesthetized fetuses were weighed and sexed. Fetal hearts were weighed and left ventricles excised and flash frozen in liquid N2 and stored in −80 οC freezer.
Extraction of Nuclear and Mitochondrial Fraction from Fetal Heart Ventricles
Frozen fetal cardiac ventricles were used to obtain nuclear and mitochondrial protein fractions for western immunoblot analysis. Briefly, 20–30 mg frozen ventricle pieces were ground with a mortar pestle in liquid N2 and resuspended in 800 μl of ice-cold homogenization buffer. The nuclear fraction was obtained by using a modified method with two-time homogenization and centrifugation [27,28,29]. The pellet containing the nuclear fraction was resuspended in 1x RIPA Lysis Buffer (Millipore, Calbiochem, MA, USA) and supplemented with 1x protease and phosphatase inhibitor cocktail tablet (Roche Diagnostics, Munich, Germany). The mitochondrial fraction was isolated by a standard differential centrifugation method [11, 13]. The pellet containing the mitochondrial fraction was resuspended in 1x RIPA Lysis Buffer (Millipore) and supplemented with 1x protease inhibitor cocktail tablet (Roche). All sample protein concentrations were measured by using the Bio-Rad Protein Assay (Bio-Rad). These procedures generate nuclear and mitochondrial fractions [30] without contamination.
Western Immunoblot
Protein expression was measured for nuclear fractions of PGC1α, SIRT1, phosphorylated-AMPK, total AMPK, and mitochondrial fractions of SIRT3. 20–30μg of total protein from either nuclear or mitochondrial fractions were loaded onto precast 4–12% Bis-Tris mini gels (Invitrogen, Waltham, MA) for gel electrophoresis and then transferred to a PVDF membrane. Nuclear proteins were detected by anti-PGC1α (1:1000), anti-SIRT1 (1:1000, Proteintech, Rosemont, IL), anti-AMPKa (1:1000), and anti-phospho-AMPK (Thr172) (1:1000, Cell Signaling Technology, Danvers, MA). Density values of each of the bands were normalized to their corresponding loading control, Lamin A/C (4C11) (1:2000, Cell Signaling Technology), and expressed as relative expression. Mitochondrial proteins were detected by anti-SIRT3 (1:1000, Abcam, Cambridge, MA) and anti-acetylated-lysine (Ac-K2-100) (1:1000, Cell Signaling Technology). Each of the bands was normalized to VDAC1/Porin (1:1000, Abcam) as a loading control and expressed as relative expression. A peroxidase-conjugated secondary antibody (SeraCare Life Sciences, Gaithersburg, MD) was used for all immunoblots.
Immunoprecipitation was performed to confirm respiratory complex I subunit was the acetylated mitochondrial protein at MW 20kDa. Mitochondrial protein was isolated from fetal heart left ventricle, and immunoprecipitation was performed using Dynabeads Protein A Immunoprecipitation Kit (Invitrogen, Waltham, MA) following the manufacturer’s protocol. Briefly, anti-acetylated-lysine (Ack) antibody at 1:100 dilution (Cell Signaling Technology) was mixed with 50 μl of Dynabeads and then incubated with 100 μl of protein lysate overnight. Lysates containing acetylated mitochondrial protein were probed with anti-NDUFB8 antibody (anti-complex I subunit, Abcam) at 1:20 dilution.
Sirtuin Activity Assay
SIRT3 enzyme activity of mitochondrial fractions was measured using the SIRT3 Activity Assay Kit (Fluorometric, Abcam, Cambridge, MA) per the manufacturer’s protocol. Briefly, 50μg of mitochondrial protein was added into individual microplate wells containing a designated amount of fluorescence-labeled acetylated substrate peptide, nicotinamide adenine dinucleotide (NAD), and the developer. Fluorescence intensity was measured (excitation at 350 nm/emission at 450 nm) for 30 min at 1-min intervals by the microplate reader (BioTek, Winooski, VT). Enzyme activity rate was calculated as ΔOD/min.
Statistical Analysis
Data are expressed as means ± SE. Each N value represents a single fetus. A total number of 20 NMX, 15 early-onset HPX, and 9 late-onset HPX pregnant sows were used to obtain the same number of male and female fetuses, respectively. Fetal heart tissue from the same fetuses were used for quantification of nuclear PGC1α, SIRT1, and SIRT3 expression. Additional animals were used for assays of SIRT3 activity and AMPK because of the limitation of tissue availability for all assays. Fetal body weight characteristics were generated from all of the fetuses used in the study. Statistical analysis was performed using Systat software (San Jose, CA). Comparisons of fetal body and organ weights were made using two-way analysis of variance (ANOVA) using the same NMX group as control. If significant effects were detected (P<0.05), post hoc analysis using the Holm-Sidak method was performed to identify differences between groups. Comparisons between protein expression and SIRT3 activity rate were made using Student’s t test because only two groups were run on a single gel and comparisons were not made between gels.
Results
Effects of HPX on Fetal Body and Heart Weights
Both early- and late-onset hypoxia significantly reduced fetal body weight (P=0.008 and P=0.006, respectively), and increased relative placental weight (placental wt/body wt ratios) (P<0.001 for both) independent of sex compared to age-matched normoxic controls (Table 1). In addition, both early- and late-onset hypoxia significantly increased relative brain weight (P<0.001 and P=0.04, respectively) similarly between males and females compared to their respective normoxic controls while relative heart weight was unchanged. This is characteristic of asymmetric fetal growth restriction, established in our animal model [13]. Neither food nor water intake rates are affected by intrauterine hypoxia [13], indicating that the fetal growth restriction induced by hypoxia in our animal model is not due to nutrient deficiency, but rather an effect on placental function [30, 31] and/or on fetal growth mechanisms [32].
Expression of Nuclear Protein Expression with Early- and Late-Onset Hypoxia
Nuclear PGC1α, SIRT1 (Fig. 1), and p-AMPK and total AMPK levels (Fig. 2) were measured in normoxic and hypoxic male and female fetal heart ventricles. Early-onset hypoxia significantly increased nuclear PGC1α in both male (p<0.001) and female (p=0.04) hearts. Nuclear SIRT1 levels were decreased with early-onset hypoxia in male (p=0.004) but not female hearts. Activated nuclear AMPK levels, measured as ratios of p-AMPK/total AMPK, were unaffected by early-onset hypoxia compared to normoxic controls. Although total AMPK levels were highly expressed in the nuclear fractions there was considerable variability in expression of the p-AMPK in both normoxic and hypoxic fetal hearts.
In contrast, late-onset hypoxia had no effect on nuclear PGC1α levels in male hearts but significantly decreased expression of both PGC1α (p=0.004) and SIRT1 (p=0.05) in female hearts (Fig. 3). There was no effect of hypoxia on the p-AMPK/total AMPK ratios in either male or female heart tissues (Fig. 4).
Expression of Mitochondrial Protein Expression with Early- and Late-Onset Hypoxia
SIRT3 is a mitochondrion-associated deacetylase important in regulating acetylation of mitochondrial proteins such as complex I and IV subunits, among others [33, 34]. Early-onset hypoxia increased both mitochondrial SIRT3 expression and the activity rate (p=0.003 and p=0.01, respectively) in male fetal hearts but had no effect in female hearts (Fig. 5). Figure 6 illustrates acetylation of mitochondrial proteins of fetal hearts was identified as a strong band at 20kDa MW similar to that for respiratory complex I, while there was no corresponding band at CIV subunit (not shown) [13]. Immunoprecipitation (inset Fig. 8) confirms that the acetylated band at 20kDa MW corresponds to complex I subunit (NDUFB8). Additional bands were only able to be visualized at longer exposure times but were faint and unable to be quantified. Early-onset hypoxia had no effect on mitochondrial acetylation in either male or female hearts.
Late-onset hypoxia significantly increased mitochondrial SIRT3 protein expression levels in both male (p<0.005) and female (p=0.01) hearts (Fig. 7). However, hypoxia inhibited SIRT3 activity (p=0.03) in male hearts only. In contrast to early-onset, late-onset hypoxia significantly (p<0.05) increased acetylation of mitochondrial proteins in hearts of both males (p=0.001) and females (p<0.001) (Fig. 8), which corresponded to respiratory complex subunit I (NDUFB8).
Discussion
Intrauterine hypoxia generates oxidative stress [4, 18, 35, 36], inhibits mitochondrial biogenesis and bioenergetics [37, 38], and disrupts normal fetal heart development [16, 39,40,41,42]. Fetal responses to chronic hypoxia include asymmetric fetal growth restriction and placental insufficiency, as well as, redistribution of its cardiac output to critical organs [36], and altered energy metabolism of fetal organs [37].
The first part of the study focused on the effects of hypoxia on nuclear PGC1α, a regulator of mitochondrial biogenesis, and nuclear SIRT1 and AMPK as regulators of PGC1α activity to determine whether chronic hypoxia alters the expression of upstream regulators in a similar direction as downstream targets such as mitochondrial respiratory complex subunits [13]. Effects of hypoxia on PGC1α expression can vary depending on the cell type, redox status of the cell, the presence of inflammation, and severity/duration of hypoxia [43], all of which can occur in hypoxic heart tissue. We previously reported increased expression of respiratory complex subunits (I, III, V) measured with early-onset hypoxia in male fetal hearts and decreased expression of the same subunits with late-onset hypoxia in fetal heart ventricles of both sexes under identical conditions [13] (see Fig. 9). In early-onset hypoxia, the increased PGC1α expression in male fetal hearts corresponded to a compensatory increase in respiratory complex subunits, despite a lack of change in either SIRT1 or activated-AMPK expression. We expected the levels of both of these proteins to be changed in a similar direction as PGC1α. However, nuclear SIRT1 levels were paradoxically decreased with hypoxia and AMPK levels were unchanged. In hypoxic female hearts, early-onset hypoxia increased PGC1α expression but to a lesser degree compared to males, which may account for the lack of change measured in mitochondrial complex subunit expression. In late-onset hypoxia, PGC1α expression was not increased, but either unchanged in male or decreased in female hearts, corresponding to the decreased mitochondrial respiratory complex subunit expression measured in both sexes [13]. In other tissue types, hypoxia increased PCG1α expression in fetal adipose tissue from high altitude pregnant sheep [44], decreased levels in hypoxic cardiomyocyte [45] and adipocyte [46] cell cultures, and decreased expression in chronically (2 and 4 weeks) hypoxic adult mice diaphragm but not skeletal muscle [47]. The current study provides new evidence that intrauterine hypoxia differentially disrupts PGC1α expression in the fetal heart ventricle depending on the timing of gestation and/or duration of hypoxia.
The regulation of downstream mitochondrial biogenesis by PGC1α is complex. Both nuclear- and mitochondrial-encoded proteins are involved in the synthesis, transport, and import into the mitochondria for assembly into respiratory chain complexes [19] via PGC1α signaling. Its expression/activity is regulated within the nucleus [19] by several processes including phosphorylation/acetylation and HIF-1 signaling [48, 49], which increase binding to DNA promoter regions [19] and induce transcription of mitochondrial proteins (i.e., transcription factors NRF1/2, TFAM), as well as, PGC1α itself. A limitation of the study is that a distinct expression pattern of nuclear and mitochondrial protein signaling is difficult to causally link. However, the trends in the overall group of data provide some insight into the significance of the directional changes in expression that occurred with hypoxia. The increased PGC1α signaling induced by early-onset hypoxia may be an adaptive response for preventing the decrease in the mitochondrial complex subunit expression and/or respiratory function in response to hypoxia [13]. In late-onset hypoxia, the lack of increase or decrease in PGC1α signaling is associated with decreased respiratory complex subunit expression, resulting in fetuses more vulnerable to cardiac mitochondrial dysfunction. This has implications regarding postnatal consequences in the programmed offspring. Hearts of prenatally hypoxic (late-onset) guinea pig male offspring exhibit downregulation of mitochondrial respiratory chain complex subunits (CI, CIII, CV) in both ventricular tissue and isolated cardiomyocytes, as well as, decreased respiratory function (i.e., maximal oxygen consumption, respiratory reserve capacity), compared to their normoxic age-matched controls [12]. In the same study [12], prenatal hypoxia reduces contractile function (e.g., stroke volume, cardiac output, ejection fraction, fractional shortening) measured by ultrasound of offspring hearts [12]. Both studies, combined, suggest an important programming effect of intrauterine hypoxia on disruption of PGC1α signaling and mitochondrial protein expression in fetal hearts with consequences manifest in the offspring. Yet, prenatally hypoxic female offspring hearts did not exhibit sustained effects on either contractile or mitochondrial function compared to males, despite hypoxic effects on PGC1α signaling and mitochondrial protein expression in female fetal hearts. Thus, there may be secondary environmental responses, postnatally, that are adaptive in female offspring.
The second part of the study investigated the effects of hypoxia on mitochondrial SIRT3 expression/activity and protein acetylation. Mitochondrial acetylation reduces mitochondrial function via inhibiting ATP generation, hormone synthesis, and calcium regulation [50]. SIRT3 is a mitochondrial deacetylase encoded in the nucleus, transported to and imported into the mitochondria where it regulates acetylation of mitochondrial proteins [51, 52] such as complexes I, II, and IV [31, 32, 53]. With late-onset hypoxia, the increased mitochondrial acetylation corresponds to the decrease in SIRT3 activity in males or no change in females. The compensatory increase in SIRT3 expression may limit the effects of SIRT3 activity although not sufficient enough to prevent the increased acetylation. An alternative may be that other mitochondrial SIRTs (i.e., SIRT4, SIRT5) [54] whose activities may be decreased by hypoxia contribute to the increased acetylation levels. Interestingly, the increased acetylation is associated with respiratory complex I subunit (NDUFB8), which SIRT3 has been reported to deacetylate [55]. In contrast, early-onset hypoxia did not increase mitochondrial acetylation in either sex. In males, there was a greater increase in SIRT3 expression compared to late-onset hypoxia along with increased activity, which may contribute to a protective response in preventing increased acetylation. Overall, increased mitochondrial acetylation, which targets complex I, imposes a great risk to mitochondrial respiration in hypoxic fetal hearts due to its potential inhibitory actions on the respiratory chain [31, 55].
Sex differences in fetal cardiac protein expression occurred in response to chronic hypoxia with regard to PGC1α and SIRT3, along with SIRT3 activity. The combined increase in levels of PGC1α, SIRT3 expression/activity, and mitochondrial respiratory complex subunits in early-onset hypoxic male but not female hearts identifies a compensatory capacity that is somewhat sex-related. With late-onset hypoxia, however, PGC1α was decreased in females but not males although both sexes increased SIRT3 expression, mitochondrial acetylation, and decreased respiratory complex subunit expression [13]. The mechanisms underlying sex differences between fetuses and adults differ, with the former relying on genetic and/or epigenetic influences [56, 57]. Mitochondria of adult female hearts exhibit a greater functional advantage over mitochondria from males because of a greater antioxidant capacity, lower generation of reactive oxygen species, greater energy production, and lower calcium uptake [56, 58]. This is attributed, in part, to a hormonal effect of estrogen on mitochondrial function and biogenesis, regulated by binding to both ERα in the nucleus and ERβ in the mitochondrion [59, 60]. While we did not evaluate baseline sex differences, sex-related responses to hypoxia appear compensatory with early-onset and decompensatory with late-onset hypoxia, regarding PGC1α signaling, SIRT1 expression/activity and respiratory complex subunit expression.
Overall, exposure to hypoxia in early gestation initiates adaptive mechanisms that protect the fetal heart with regard to mitochondrial respiration prior to birth or has a lesser impact due to reduced mitochondrial maturity [6, 61]. The cardiac response to hypoxia in late gestation, however, shows a decompensation with no change or decreased PCC1α signaling, decreased mitochondrial respiratory subunit expression [13], and increased mitochondrial acetylation. The reduced capacity of fetal hearts to adaptively respond to hypoxia in late gestation may be due to a shorter time interval and/or a reduced plasticity of cellular mechanisms for compensation. This identifies a differential capacity of the fetal heart mitochondria to respond to chronic hypoxia depending on the conditions, which may increase the risk of mitochondrial dysfunction, contributing to cardiovascular programming of the offspring [15, 57].
References
Aye ILMH, Aiken CE, Charnock-Jones DS, Smith GCS. Placental energy metabolism in health and disease—significance of development and implications for preeclampsia. Am J Obstet Gynecol. 2022;226(2S):S928–44.
Giussani DA. The fetal brain sparing response to hypoxia: physiological mechanisms. J Physiol. 2016;594(5):1215–30. https://doi.org/10.1113/JP271099.
Fuhrmann DC, Brüne B. Mitochondrial composition and function under the control of hypoxia. Redox Biol. 2017;12:208–15. https://doi.org/10.1016/j.redox.2017.02.012.
Hu X-Q, Zhang L. Hypoxia and mitochondrial dysfunction in pregnancy complications. Antioxidants (Basel). 2021;10(3):405. https://doi.org/10.3390/antiox10030405.
Piquereau J, Ventura-Clapier R. Maturation of cardiac energy metabolism during perinatal development. Front Physiol. 2018;19(9):959. https://doi.org/10.3389/fphys.2018.00959.
Rolph TP, Jones CT, Parry D. Ultrastructural and enzymatic development of fetal guinea pig heart. Am J Physiol. 1982;243(1):H87–93. https://doi.org/10.1152/ajpheart.1982.243.1.H87.
Morrison JL, Botting KJ, Darby JRT, David AL, Dyson RM, Gatford KL, Gray C, Herrera EA, Hirst JJ, Kim B, Kind KL, Krause BJ, Matthews SG, Palliser HK, Regnault TRH, Richardson BS, Sasaki A, Thompson LP, Berry MJ. Guinea pig models for translation of the developmental origins of health and disease hypothesis into the clinic. J Physiol. 2018;596(23):5535–69. https://doi.org/10.1113/JP274948.
Hoerter JA, Ventura-Clapier R, Kuznetsov A. Compartmentation of creatine kinases during perinatal development of mammalian heart. Mol Cell Biochem. 1994;133-134:277–86. https://doi.org/10.1007/BF01267960.
Gilbert RD. Fetal myocardial responses to long-term hypoxemia. Comp Biochem Physiol A Mol Integr Physiol. 1998;119(3):669–74. https://doi.org/10.1016/s1095-6433(98)01003-4.
Gilbert RD, Pearce WJ, Longo LD. Fetal cardiac and cerebrovascular acclimatization responses to high altitude, long-term hypoxia. High Alt Med Biol. 2003;4(2):203–13. https://doi.org/10.1089/152702903322022802.
Al-Hasan YM, Evans LC, Pinkas GA, Dabkowski ER, Stanley WC, Thompson LP. Chronic hypoxia impairs cytochrome oxidase activity via oxidative stress in selected fetal guinea pig organs. Reprod Sci. 2013;20(3):299–307.
Thompson LP, Chen L, Polster BM, Pinkas G, Song H. Prenatal hypoxia impairs cardiac mitochondrial and ventricular function in guinea pig offspring in a sex-related manner. Am J Physiol Regul Integr Comp Physiol. 2018;315(6):R1232–41.
Song H, Polster BM, Thompson LP. Chronic hypoxia alters cardiac mitochondrial complex protein expression and activity in fetal guinea pigs in a sex-selective manner. Am J Physiol Regul Integr Comp Physiol. 2021;321(6):R912–24. https://doi.org/10.1152/ajpregu.00004.2021.
Smith KLM, Swiderska A, Lock MC, Graham L, Iswari W, Choudhary T, Thomas D, Kowash HM, Desforges M, Cottrell EC, Trafford AW, Giussani DA, Galli GLJ. Chronic developmental hypoxia alters mitochondrial oxidative capacity and reactive oxygen species production in the fetal rat heart in a sex-dependent manner. J Pineal Res. 2022;73(3):e12821. https://doi.org/10.1111/jpi.12821.
Zhang L. Prenatal hypoxia and cardiac programming. J Soc Gynecol Investig. 2005;12(1):2–13. https://doi.org/10.1016/j.jsgi.2004.09.004.
Patterson AJ, Zhang L. Hypoxia and fetal heart development. Curr Mol Med. 2010;10(7):653–66. https://doi.org/10.2174/156652410792630643.
Nuyt AM, Alexander BT. Developmental programming and hypertension. Curr Opin Nephrol Hypertens. 2009;18(2):144–52. https://doi.org/10.1097/MNH.0b013e328326092c.
Giussani DA, Davidge ST. Developmental programming of cardiovascular disease by prenatal hypoxia. J Dev Orig Health Dis. 2013;4(5):328–37. https://doi.org/10.1017/S204017441300010X.
Brenmoehl J, Hoeflich A. Dual control of mitochondrial biogenesis by sirtuin 1 and sirtuin 3. Mitochondrion. 2013;13(6):755–61. https://doi.org/10.1016/j.mito.2013.04.002.
Lehman JJ, Barger PM, Kovacs A, Saffitz JE, Medeiros DM, Kelly DP. Peroxisome proliferator-activated receptor gamma coactivator-1 promotes cardiac mitochondrial biogenesis. J Clin Invest. 2000;106(7):847–56. https://doi.org/10.1172/JCI10268.
Puigserver P, Speigelman BM. Peroxisome proliferator-activated receptor-gamma coactivator 1 alpha (PGC1-alpha): transcriptional coactivator and metabolic regulator. Endocr Rev. 2003;24:78–90.
Hock MB, Kralli A. Transcriptional control of mitochondrial biogenesis and function Annu. Rev. Physio. 2009;71:177–203.
Hallows WC, Lee S, Denu JM. Sirutins deacetylate and activate mammalian acetyl-CoA synthetases. Proc Natl Acad Sci USA. 2006;103:10230–5.
Thompson L, Dong Y, Evans L. Chronic hypoxia increases inducible NOS-derived nitric oxide in fetal guinea pig hearts. Pediatr Res. 2009;65:188–92.
Evans LC, Liu H, Pinkas GA, Thompson LP. Chronic hypoxia increases peroxynitrite, MMP9 expression, and collagen accumulation in fetal guinea pig hearts. Ped Res. 2012;71(1):25–31.
Kaufmann P, Davidoff M. The guinea-pig placenta. Adv Anat Embryol Cell Biol. 1977;53:5–91.
Bergmann O, Jovinge S. Isolation of cardiomyocyte nuclei from post-mortem tissue. J Vis Exp. 2012;65:e4205. https://doi.org/10.3791/4205.
Lozano S. Human heart nuclei isolation for DroNc-seq, vol. 2. Protocols.io; 2018. https://doi.org/10.17504/protocols.io.vgue3ww.
Wang S-B, Venkatraman V, Crowgey EL, Liu T, Fu Z, Holewinski R, Ranek M, Kass DA, O’Rourke B, Van Eyk JE. Protein S-nitrosylation controls glycogen synthase kinase 3β function independent of its phosphorylation state. Circ Res. 2018;122:1517–31. https://doi.org/10.1161/CIRCRESAHA.118.312789.
Song H, Telugu BP, Thompson LP. Sexual dimorphism of mitochondrial function in the hypoxic guinea pig placenta. Biol Reprod. 2019;100(1):208–16. https://doi.org/10.1093/biolre/ioy167.
Määttä J, Sissala N, Dimova EY, Serpi R, Moore LG, Koivunen P. Hypoxia causes reductions in birth weight by altering maternal glucose and lipid metabolism. Sci Rep. 2018;8(1):13583. https://doi.org/10.1038/s41598-018-31908-2.
Hutter D, Kingdom J, Jaeggi E. Causes and mechanisms of intrauterine hypoxia and its impact on the fetal cardiovascular system: a review. Int J Pediatr. 2010;2010:401323. https://doi.org/10.1155/2010/401323.
Bause AS, Haigis MC. SIRT3 regulation of mitochondrial oxidative stress. Exp Gerontol. 2013;48(7):634–9. https://doi.org/10.1016/j.exger.2012.08.007.
Cortés-Rojo C, Vargas-Vargas MA, Olmos-Orizaba BE, Rodríguez-Orozco AR, Calderón-Cortés E. Interplay between NADH oxidation by complex I, glutathione redox state and sirtuin-3, and its role in the development of insulin resistance. Biochim Biophys Acta Mol Basis Dis. 2020;1866(8):165801. https://doi.org/10.1016/j.bbadis.2020.165801.
Giussani DA, Camm EJ, Niu Y, Richter HG, Blanco CE, Gottschalk R, Blake EZ, Horder KA, Thakor AS, Hansell JA, Kane AD, Wooding FB, Cross CM, Herrera EA. Developmental programming of cardiovascular dysfunction by prenatal hypoxia and oxidative stress. PLoS One. 2012;7(2):e31017. https://doi.org/10.1371/journal.pone.0031017.
Giussani DA, Niu Y, Herrera EA, Richter HG, Camm EJ, Thakor AS, Kaen AD, Hansel JA, Brain KL, Skeffingtonn KL, Itani N, Wooding FBP, Cross CM, Allison BJ. Heart disease link to fetal hypoxia and oxidative stress. In: Zhang L, Ducsay C, editors. Advances in fetal and neonatal physiology, vol. 814. New York, NY: Springer; 2014. https://doi.org/10.1007/978-1-4939-1031-1_7.
El Azzouzi H, Leptidis S, Doevendans PA, De Windt LJ. HypoxamiRs: regulators of cardiac hypoxia and energy metabolism. Trends Endocrinol Metab. 2015;26(9):502–8.
McLeod CJ, Pagel I, Sack MN. The mitochondrial biogenesis regulatory program in cardiac adaptation to ischemia—a putative target for therapeutic intervention. Trends Cardiovasc Med. 2005;15(3):118–23. https://doi.org/10.1016/j.tcm.2005.05.001.
Botting KJ, McMillen IC, Forbes H, Nyengaard JR, Morrison JL. Chronic hypoxemia in late gestation decreases cardiomyocyte number but does not change expression of hypoxia-responsive genes. J Am Heart Assoc. 2014;3(4):e000531.
Botting KJ, Loke XY, Zhang S, Andersen JB, Nyengaard JR, Morrison JL. IUGR decreases cardiomyocyte endowment and alters cardiac metabolism in a sex- and cause-of-IUGR-specific manner. Am J Physiol Regul Integr Comp Physiol. 2018;315(1):R48–67. https://doi.org/10.1152/ajpregu.00180.2017.
Thornburg K, Jonker S, O'Tierney P, Chattergoon N, Louey S, Faber J, Giraud G. Regulation of the cardiomyocyte population in the developing heart. Prog Biophys Mol Biol. 2011;106(1):289–99. https://doi.org/10.1016/j.pbiomolbio.2010.11.010.
Ducsay CA, Goyal R, Pearce WJ, Wilson S, Hu X-Q, Zhang L. Gestational hypoxia and developmental plasticity. Physiol Rev. 2018;98(3):1241–334. https://doi.org/10.1152/physrev.00043.2017.
Hadanny A, Efrati S. The hyperoxic-hypoxic paradox. Biomolecules. 2020;10(6):958. https://doi.org/10.3390/biom1006095.
Myers DA, Hanson K, Mlynarczyk M, Kaushal KM, Ducsay CA. Long-term hypoxia modulates expression of key genes regulating adipose function in the late-gestation ovine fetus. Am J Physiol Regul Integr Comp Physiol. 2008;294(4):R1312–8. https://doi.org/10.1152/ajpregu.00004.2008.
Rabinovich-Nikitin I, Blant A, Dhingra R, Kirshenbaum LA, Czubryt MP. Cells NF-κB p65 attenuates cardiomyocyte PGC-1α expression in hypoxia. J Mol Cell Cardiol. 2022;11(14):2193. https://doi.org/10.3390/cells11142193.
Yun Z, Maecker HL, Johnson RS, Giaccia AJ. Inhibition of PPAR gamma 2 gene expression by the HIF-1-regulated gene DEC1/Stra13: a mechanism for regulation of adipogenesis by hypoxia. Dev Cell. 2002;2(3):331–41. https://doi.org/10.1016/s1534-5807(02)00131-4.
Gamboa JL, Andrade FH. Mitochondrial content and distribution changes specific to mouse diaphragm after chronic normobaric hypoxia. Am J Physiol Regul Integr Comp Physiol. 2010;298(3):R575–83. https://doi.org/10.1152/ajpregu.00320.2009.
Wentz T. Regulation of mitochondrial biogenesis and PGC-1α under cellular stress. Mitochondrion. 2013;13:134–42.
Taylor CT. Mitochondria and cellular oxygen sensing in the HIF pathway. Biochem J. 2008;409:19–26.
Lopaschuk GD, Karwi OG, Tian R, Wende AR, Abel ED. Cardiac energy metabolism in heart failure. Circulation Research. 2021;128(10):1487–513.
Lin L, Chen K, Khalek WA, Ward JL 3rd, Yang H, Chabi B, Wrutniak-Cabello C, Tong Q. Regulation of skeletal muscle oxidative capacity and muscle mass by SIRT3. PLoS One. 2014;9(1):e85636. https://doi.org/10.1371/journal.pone.0085636.
Giralt A, Villarroya F. SIRT3, a pivotal actor in mitochondrial functions: metabolism, cell death and aging. Biochem J. 2012;444(1):1–10. https://doi.org/10.1042/BJ20120030.
Foster DB, Liu T, Rucker J, O'Meally RN, Devine LR, Cole RN, O'Rourke B. The cardiac acetyl-lysine proteome. PLoS One. 2013;8(7):e67513. https://doi.org/10.1371/journal.pone.0067513.
Huang JW, Hirschey MD, Shimazu T, Ho L, Verdin E. Mitochondrial sirtuins. Biochim. Biophys. Acta. 2010;1804:1645–16521.
Ahn B-H, Kim H-S, Song S, Lee IH, Liu J, Vassilopoulos A, Deng C-X, Finkel T. A role for the mitochondrial deacetylase Sirt3 in regulating energy homeostasis. Proc Natl Acad Sci USA. 2008;105(38):1447–14452.
Ventura-Clapier R, Dworatzek E, Seeland U, Kararigas G, Arnal J-F, Brunelleschi S, Carpenter TC, Erdmann JF, Giannetta E, Glezerman M, Hofmann SM, Junien C, Katai M, Kublickiene K, König IR, Majdic G, Malorni W, Mieth C, Miller VM, et al. Sex in basic research: concepts in the cardiovascular field. Cardiovasc Res. 2017;113(7):711–24. https://doi.org/10.1093/cvr/cvx066.
Chen M, Zhang L. Epigenetic mechanisms in developmental programming of adult disease. Drug Discov Today. 2011;16(23-24):1007–18. https://doi.org/10.1016/j.drudis.2011.09.008.
Ventura-Clapier R, Piquereau J, Garnier A, Mericskay M, Lemaire C, Crozatier B. Gender issues in cardiovascular diseases. focus on energy metabolism. Biochim Biophys Acta Mol Basis Dis. 2020;1866(6):165722. https://doi.org/10.1016/j.bbadis.2020.165722.
Chen JQ, Cammarata PR, Baines CP, Yager JD. Regulation of mitochondrial respiratory chain biogenesis by estrogens/estrogen receptors and physiological, pathological and pharmacological implications. Biochim Biophys Acta. 2009;1793(10):1540–70. https://doi.org/10.1016/j.bbamcr.2009.06.001.
Klinge CM. Estrogenic control of mitochondrial function. Redox Biol. 2020;31:101435. https://doi.org/10.1016/j.redox.2020.101435.
Yanicostas C, Soussi-Yanicostas N, El-Khoury R, Bénit P, Rustin P. Developmental aspects of respiratory chain from fetus to infancy. Semin Fetal Neonatal Med. 2011;16(4):175–80. https://doi.org/10.1016/j.siny.2011.05.005.
Acknowledgements
The content is solely the responsibility of the authors and does not necessarily represent the official view of the National Institutes of Health.
Funding
The project described is supported in part by a National Institute of Health (NIH HL126859, LPT) grant.
Author information
Authors and Affiliations
Corresponding author
Ethics declarations
Ethics Approval
All animal procedures were approved by the University of Maryland Animal Care and Use Committee in accordance with the Association for Assessment and Accreditation of Laboratory Animal Care- accredited procedures (Animal Welfare Assurance No. A3200-01).
Conflict of Interest
The authors declare no competing interests.
Additional information
Publisher’s Note
Springer Nature remains neutral with regard to jurisdictional claims in published maps and institutional affiliations.
Rights and permissions
Open Access This article is licensed under a Creative Commons Attribution 4.0 International License, which permits use, sharing, adaptation, distribution and reproduction in any medium or format, as long as you give appropriate credit to the original author(s) and the source, provide a link to the Creative Commons licence, and indicate if changes were made. The images or other third party material in this article are included in the article's Creative Commons licence, unless indicated otherwise in a credit line to the material. If material is not included in the article's Creative Commons licence and your intended use is not permitted by statutory regulation or exceeds the permitted use, you will need to obtain permission directly from the copyright holder. To view a copy of this licence, visit http://creativecommons.org/licenses/by/4.0/.
About this article
Cite this article
Song, H., Thompson, L.P. Effects of Gestational Hypoxia on PGC1α and Mitochondrial Acetylation in Fetal Guinea Pig Hearts. Reprod. Sci. 30, 2996–3009 (2023). https://doi.org/10.1007/s43032-023-01245-5
Received:
Accepted:
Published:
Issue Date:
DOI: https://doi.org/10.1007/s43032-023-01245-5