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Frontiers in Cellular and Infection Microbiology logoLink to Frontiers in Cellular and Infection Microbiology
. 2021 Aug 23;11:671347. doi: 10.3389/fcimb.2021.671347

Maternal Obesity Increases Oxidative Stress in Placenta and It Is Associated With Intestinal Microbiota

Chengjun Hu 1,†, Yingli Yan 1,†, Fengjie Ji 1, Hanlin Zhou 1,*
PMCID: PMC8420882  PMID: 34497775

Abstract

Maternal obesity induces placental dysfunction and intestinal microbial dysbiosis. However, the associations between intestinal microbiota and placental dysfunction are still unclear. In the present study, a gilt model was used to investigate the role of maternal obesity on placental oxidative stress, mitochondrial function, and fecal microbiota composition, meanwhile identifying microbiota markers associated with placental oxidative stress. Twenty gilts were divided into two groups based on their backfat thickness on parturition day: namely Con group (average backfat thickness = 33 mm), and Obese group (average backfat thickness = 39 mm). The results showed that Obese group was lower than Con group in the birth weight of piglets. Compared with the Con group, the Obesity group exhibited an increased oxidative damage and inflammatory response in placenta, as evidenced by the increased concentrations of placental reactive oxygen species (ROS), protein carboxyl, and interleukin-6 (IL-6). Obesity group was lower than Con group in the concentrations of placental adenosine triphosphate, citrate synthase, and complex I activity. In addition, lower propionate level and Bacteroidetes abundance in feces were seen in the Obese Group. Furthermore, the concentrations of placental ROS, protein carboxyl, and IL-6 were positively correlated with the abundance of Christensenellaceae_R-7_group and negatively correlated with that of norank_f_Bacteroidales_S24-7_group. In conclusion, these findings suggest that maternal obesity might impair oxidative and inflammatory response in placenta through modulating intestinal microbiota composition.

Keywords: intestinal microbiota, mitochondrial biogenesis, obesity, oxidative stress, placenta

Introduction

Over the past few decades, the incidence of obesity has increased dramatically worldwide (Ng et al., 2014), which is one of the major risk factors for diseases, such as type-2 diabetes, inflammation, and cardiovascular diseases (Zhang et al., 2018). Specially, the prevalence of obesity among women is higher than that among men, which is 40.4% compared with 35% (Tauqeer et al., 2018). The number of obese or overweight women even increases during pregnancy, which induces placental dysfunction (Myatt and Maloyan, 2016; Godfrey et al., 2017). However, its mechanisms are still unclear.

Gut microbiota plays a vital role in the placental development. For instance, through transferring the microbiota from patients with pre-eclampsia to mice, the ratio of labyrinth and junctional zones was increased and the placental weight was decreased (Chen et al., 2020). However, with the current evidence, the change of placental function contributed by bacterial species is still unclear. Short-chain fatty acids (SCFAs), products of intestinal microbiota, not only serve as an energy source for hosts (Zhi et al., 2019), but also play a vital role in placental development. For instance, butyrate induces trophoblast differentiation and syncytiotrophoblast formation in early gestation (Kumar et al., 2015); and propionate blocks the secretion of pro-inflammatory cytokines and chemokines in placenta (Roy et al., 2020). Given SCFAs function as a link between the microbiota and the host, understanding the dynamic changes of SCFAs in obesity will help us have a better understanding of the relationship between intestinal microbiota and placental function.

Our previous study shows that maternal obesity increases oxidative stress and impairs mitochondrial function in placenta (Hu et al., 2019a). However, the relationship among the intestinal microbiota, placental oxidative stress, inflammatory response, and mitochondrial function has not been clarified so far. Gilt is an animal commonly used in human biomedical studies (Song et al., 2018). Therefore, gilts with a high backfat thickness were used as an obesity model to capture the changed microbiota involved in placental oxidative stress in obesity.

Materials and Methods

Animals and Experimental Treatments

After mating, gilts were housed individually in a stall (1.8 × 0.7 × 1.0 m) and fed twice at 7:00 and 17:00 daily. The animals had ad libitum access to water through nipple drinkers. On parturition day, the body weight of gilts was weighed and their backfat thickness was measured at position P2 using ultrasonography (Renco Lean-Meater®, Minneapolis, MN, USA). Then the gilts were moved to the farrowing rooms and housed individually in slatted farrowing crates (2.0 m × 1.5 m). The total number of piglets born was recorded and their weight was measured within 6 h after birth. The average backfat thickness of the gilts was 36.61 ± 0.83 mm (means± standard error). Therefore, the gilts were assigned to two groups according to their backfat thickness: average backfat thickness = 33 mm (Con group) and average backfat thickness = 39 mm (Obese group) (Figure 1A).

Figure 1.

Figure 1

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Phenotype changes in gilts with different backfat thickness. Maternal backfat thickness (A) and body weight (B) at parturition day. (C) Piglet birth weight. (D) Number of piglets at birth. The concentrations of estradiol (E), progesterone (F), prolactin (G), prolactin, and FSH (H) in maternal serum. Values are mean ± SEM, n = 10. “*” and “**” indicate 0.01 < P ≤ 0.05 and 0.001 < P ≤ 0.01, respectively.

Sample Collection

Eight gilts were randomly selected from each group for sample collection. On parturition day, blood samples were collected from the ear vein through 10 mL centrifuge tubes and were centrifuged at 3,000 × g and 4°C for 15 min to obtain the serum. After the placentae were expelled, those of piglets with an average birth weight were obtained and separated from endometrium, after which about 3 g of placental samples (3 to 5 cm from the cord insertion point) were collected and quickly snap-frozen in liquid nitrogen. Colonic fecal samples were collected through massaging the rectum of those gilts on parturition day (Wang et al., 2019), which was then stored at -80°C for further analyses.

Determination of Serum Hormone Level

The concentrations of progesterone, follicle-stimulating hormone (FSH), estradiol (CSB-E06844p,Cusabio, Wuhan, China, https://www.cusabio.com/), and prolactin (SEKP-0022, Solarbio, Beijing, China) in serum were determined through Elisa kits according to the manufacturer’s instructions.

Oxidative Stress Parameters

The levels of reactive oxygen species (ROS), malondialdehyde (MDA), superoxide dismutase (SOD), glutathione (GSH), and protein carbonyl in placentae were analyzed through commercial kits (E004-1-1,A003-1-2, A001-3-2,A006-2-1, A087-1-1,Nanjing Jiancheng Bioengineering Institute, Nanjing, China) respectively.

Adenosine Triphosphate (ATP), Citrate Synthase, Complex I and III Activities

ATP level (S0026, Beyotime, Beijing, China), citrate synthase activity (A108-1-2, Nanjing Jiancheng Bioengineering Institute, Nanjing, China) as well as complex I and III activities (FHTA-2-Y, FHTC-2-Y, Cominbio Co., Suzhou, China) in placentae were determined through commercial kits. The above tests were performed according to the manufacturer’s instructions.

The Levels of Interleukin-6 (IL-6) and Tumor Necrosis Factor (TNF-α) in Placentae

The concentrations of IL-6 and TNF-α in placentae were determined using Elisa kits (CSB-E06786p, CSB-E16980p, Cusabio, Wuhan, China) according to the manufacturer’s instructions.

Short-Chain Fatty Acids (SCFAs) Concentration in Feces

The samples were analyzed through gas chromatography (Hu et al., 2019c). The feces were dissolved in dd H2O and mixed through a vortex. The solution mixture was centrifuged at 10000 rpm/min to obtain the supernatant fluid, which was mixed with 25% metaphosphoric acid solution (1 mL:0.25 mL) and was then centrifuged at 20,000 ×g and 4°C for 10 min. The supernatant was filtered through a 0.45-μm polysulfone membrane before further analyses.

Real-Time Quantitative PCR

The mRNA levels of targets genes were analyzed as we described previously (Hu et al., 2019a). Primers selected for PCR analyses are listed in Supplemental Table 1.

Western Blotting

Total protein in placentae was extracted through homogenizing and lysing in RIPA lysis buffer (P0013B, Beyotime, Shanghai, China) and its concentration was determined using BCA kits (P0009, Beyotime, Shanghai, China). Protein was separated with SDS-PAGE and blotting onto PVDF membranes. Blots were then incubated overnight at 4°C with the following primary antibodies: peroxisome proliferator-activated receptor γ coactivator-1 (PGC-1α) antibody (2178S, CST, USA) and β-Actin antibody (4970, CST, USA). The density of bands was quantified through Image J software (National Institutes of Health, Bethesda, MD).

DNA Extraction and PCR Amplification

DNA was extracted from feces samples (n = 6/group) through the HiPure Stool DNA kit B (D3141-02, Magen, Shanghai, China) according to the manufacturer’s instructions. The V3-V4 region of the 16S rRNA gene was amplified through universal primers 515F and 806R. PCR was performed as was previously described (Hu et al., 2019b). The amplified PCR products were identified through agarose gel electrophoresis. Then these products were extracted, purified through the SanPrep DNA Gel Extraction kit (B518131-0050, Sangon Biotech, Shanghai, China), and quantified through the PicoGreen dsDNA assay kit (P7581, Invitrogen, Carlsbad, CA, USA). Purified products were subject to paired-end sequencing on the Illumina MiSeq platform (Illumina, Sand Diego, CA, USA) according to a commercial service provider (Shanghai Majorbio Bio-pharm Technology Co., Ltd, Shanghai, China).

Bioinformatics Analysis

The raw Illumina fastq files were quality-filtered, de-multiplexed and analyzed through QIIME and FLASH (v1.2.11) software package to obtain an original spliced sequence. The raw tags were analyzed using Trimmomatic (v.0.30) and FLASH (v.1.2.11) software package to obtain high-quality clean reads. The criteria for low quality sequences filtration was described in our previous study (Hu et al., 2019b). The effective tags were clustered into operational taxonomic units (OTUs) with a similarity of 97% through USEARCH (v7.0.1090). Then the OTU sequences were taxonomically classified using the Ribosomal Database Project (RDP) Classifier based on the Greengene (V201305) reference database.

Alpha diversity of microbiota was estimated based on ACE, Chao 1, Simpson, and Shannon indices. The beta (β) diversity of microbiota among samples was analyzed through a principal coordinate analysis (PCoA) based on an unweighted UniFrac distance. Phylogenetic investigation of communities by reconstruction of unobserved states (PICRUSt) was employed to predict microbial functions.

Statistical Analyses

Data was presented as mean ± SEM. Statistical analyses were performed using SPSS 20.0 (SPPS Inc., Chicago, IL) software. Differences between the two groups were analyzed using student’s t-test. The relative species abundance of gut microbial communities was analyzed through the Mann-Whitney U-test. Spearman’s correlation coefficient was used to investigate the associations among backfat thickness, SCFAs level, oxidative stress parameters, and the relative abundance of microbiota. Differences were considered statistically significant at P < 0.05.

Results

Piglet Birth Weight and Maternal Serum Hormone Level

Compared to Con group, Obese group exhibited an increase in body weight of gilts (Figure 1B) and a decrease in piglet birth weight (Figure 1C). No difference was observed in the number of piglets at birth among the two groups (Figure 1D). In addition, the Obese group had a decreasing trend (P = 0.07) in the maternal serum progesterone level (Figure 1F). However, the concentrations of estradiol, prolactin, and FSH in serum (Figures 1E, G, H) showed no difference among the two groups.

Oxidative Stress Level in Placentae

As shown in Figure 2, placentae from Obese group were higher than that from Con group in the levels of ROS, MDA, and protein carbonyl (Figures 2A–C). Compared to Con group, there was an obvious decrease in the level of placental SOD in Obese group (Figure 2E). However, no difference was observed in the GSH level between Con and Obese groups (Figure 2D).

Figure 2.

Figure 2

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Oxidative stress levels in placentae. Placental ROS (A), MDA (B), protein carbonyl (C), GSH (D), and SOD (E) levels. Values are mean ± SEM, n = 8. “*” indicates statistically significant differences (P < 0.05).

Inflammatory Cytokine Level in Placentae

As shown in Figure 3, Obese group was significantly lower than Con group in the level of placental IL-6 (Figure 3A) and mRNA of IL-6 (Figure 3C). However, no difference was observed in the TNF-α level between Con and Obese groups (Figure 3D).

Figure 3.

Figure 3

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Placental inflammatory cytokine levels. (A–E) The mRNA levels of IL-6, TNF-α, IL-1β, IL-10, and IL-12 in placentae. The concentrations of IL-6 (F) and TNF-α (G) in placenta. Values are mean ± SEM, n = 8. “*” indicates statistically significant differences (P < 0.05).

Placental ATP Level and Mitochondrial Function

As shown in Figure 4, Obese group had a trend to decrease placental ATP level (Figure 4A) and was significantly lower than Con group in placental citrate synthase and complex I activity (Figures 4B, C). In addition, the protein level of PGC-1α in Obese group was lower than in Con group (Figures 4E, F).

Figure 4.

Figure 4

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Mitochondrial function in placentae. Mitochondrial function was estimated by ATP (A) level, citrate synthase (B), Complex I (C), and III (D) activities. The protein level of PGC-1α in placentae (E, F). Values are mean ± SEM, n = 8. “*” and “**” indicate P < 0.05 and < 0.01, respectively.

The Concentration of SCFAs in Feces

The concentration of SCFAs in feces was shown in Figure 5. When compared to Con group, the Obese group was seen to have a lower concentration of propionate in feces (Figure 5B). In addition, the Obese group displayed a lower trend (P = 0.09) in the concentration in the SCFAs (Figure 5D). The two groups showed no difference in the concentration of acetate or butyrate (Figures 5A, C).

Figure 5.

Figure 5

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The concentrations of SCFAs in the feces of gilts. (A–D) Fecal acetate, propionate, and butyrate concentrations, respectively. (E) Correlation analysis of serum hormone, placental immune marker, antioxidant indexes, and fecal SCFAs levels. Data represent the means ± SEM. “*”, “**”, and “***” indicate P < 0.05, < 0.01, and < 0.001, respectively.

The Spearman analysis showed that backfat thickness was negatively correlated with the concentrations of propionate, butyrate, progesterone, while was positively correlated with that of ROS, MDA, protein carboxyl, and IL-6 in placenta (Figure 5E), indicating that maternal obesity was positively correlated with placental oxidative stress.

The concentration of propionate was negatively correlated with that of protein carboxyl and IL-6 in placenta, while was positively correlated with that of progesterone. In addition, the concentration of serum progesterone was negatively correlated with that of ROS, MDA, and protein carboxyl in placenta.

Diversity of Fecal Microbiota Communities

After size filtering, quality control, and chimera removal, an average of 39, 304 and 40, 224 sequences were obtained in Con and obese groups, respectively (Supplemental Table 2). The rarefaction curves indicated that almost all bacterial species were obtained (Supplemental Figure 1). 1,158 and 1,223 OUTs were obtained in Con and obese group, respectively, 1,055 of which were shared (Supplemental Figure 2).

The PCoA analysis showed that fecal samples tended to cluster according to groups (Figure 6A). α diversity of microbiota was estimated by ACE, Chao 1, Simpson and Shannon index. Compared to the Con group, the Obese group showed a lower ACE, Chao 1, and Simpson index (Figures 6B–D). However, the 2 groups showed no difference in the Shannon index (Figure 6E).

Figure 6.

Figure 6

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Alpha and beta diversities for the fecal microbiota community. (A) Principal coordinates analysis (PCoA, Bray–Curtis distance) plot of the fecal microbial community structure. (B–E). The microbiota α diversity was estimated by ACE, Chao 1, Simpson, and Shannon index. “*” indicates statistically significant differences (P < 0.05).

Microbiota Community Composition

The most dominant phyla among microbiota communities (>1%) were Firmicutes, Bacteroidetes, Spirochaetes, Tenericutes, Actinobacteria, and Proteobacteria (Figure 7A); these microbiotas accounted for more than 96% of the total microbiota found in fecal samples. Obese group was higher than Con group in the Firmicutes: Bacteroidetes (F: B) ratio (Figure 7C). Compared to Con group, Obese group displayed a higher abundance of Firmicutes, and a lower abundance of Bacteroidetes (Figure 7D).

Figure 7.

Figure 7

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Microbial community composition. Distribution of microbiota composition at phylum (A) and genera levels (B). (C) The ratio of Firmicutes to Bacteroidetes (F: B). Comparison of relative abundance at the phylum (D) and genus (E) levels between the two groups.

Figure 7B shows the abundance of the bacterial genera (>1%) in the two groups. The most dominant genus among microbiota communities were norank_f_ Bacteroidetes_S24-7_group, Treponema_2, Lachnospiraceae_XPB1014_group, Ruminococcaceae_UCG_005, and unclassified_f_ Lachnospiraceae. The abundances of norank_f_ Bacteroidetes_S24-7_group and Alloprevotella were lower, while that of Lachnospiraceae_XPB1014_group, Ruminococcaceae_UCG-002, Streptococcus, and Christensenellaceae_R-7_group were higher, in the Obese group than in the Con group (Figure 7E). In addition, the Obese group displayed a lower trend abundance of lactobacillus and ruminococcaceae_UCG-014.

Correlation Between Microbial Community Composition, Oxidative Stress Index, Immune Marker, SCFAs, and Serum Hormone Level

At the phylum level (Figure 8A), the abundance of Firmicutes was positively correlated with backfat thickness and the concentration of IL-6 in placentae, while was negatively correlated with the concentration of SCFAs. The abundance of Bacteroidetes was negatively correlated with the concentration of protein carboxyl in placentae, and that of Proteobacteria was positively correlated with the concentrations of ROS, protein carboxyl, and IL-6 in placentae, while was negatively correlated with the concentrations of propionate and butyrate.

Figure 8.

Figure 8

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Correlations between the microbiota, backfat thickness, short-chain fatty acids, and hormone levels. Correlation analysis at the phylum (A) and genera (B) levels. “*”, “**”, and “***” indicate P < 0.05, < 0.01,and < 0.001 respectively.

At the genus level (Figure 8B), the abundance of Christensenellaceae_R-7_group was positively correlated with backfat thickness, the concentrations of ROS, protein carboxyl, and IL-6. The abundance of Ruminococcaceae_UCG-005 was positively correlated with backfat thickness and the concentration of protein carboxyl, while that of norank_f:Bacteroidales_S24-7_group was negatively correlated with backfat thickness, the concentrations of placental ROS, protein carboxyl and IL-6. These results suggest that maternal obesity was positively correlated with the abundance of Ruminococcaceae_UCG-005, but negatively correlated with the abundance of norank_f_Bacteroidales_S24-7_group.

Function Prediction of Microbiota Communities

PICRUSt was used to estimate the function of the fecal microbiota in gilts of the Con and Obese group. As shown in Table 1, microbiota from Obese gilts had a lower trend (P = 0.09) abundance of energy production and conversion, and displayed lower abundances of carbohydrate transport, metabolism, amino acid transport, and metabolism than that of gilts in the Con group.

Table 1.

PICRUSt analysis of predictive metagenomics function of the fecal microbiota.

Description CON Obese P-value
Translation, ribosomal structure, and biogenesis 4084414 ± 153262 3997426 ± 153313 0.70
RNA processing and modification 154 ± 22 389 ± 81 0.02
Transcription 2904158 ± 177021 3129631 ± 140965 0.34
Replication, recombination, and repair 2649832 ± 109236 2617864 ± 106529 0.84
Chromatin structure and dynamics 794 ± 111 998 ± 130 0.26
Cell cycle control, cell division, chromosome partitioning 602493 ± 26095 585050 ± 26259 0.65
Defense mechanisms 1096506 ± 55118 1120853 ± 44694 0.74
Signal transduction mechanisms 1643514 ± 64697 1664604 ± 63506 0.82
Cell wall/membrane/envelope biogenesis 3157429 ± 96701 2793209 ± 109657 0.03
Cell motility 437506 ± 31128 512648 ± 16134 0.06
Cytoskeleton 672 ± 146 967 ± 66 0.10
Extracellular structures 7 ± 3 5 ± 3 0.60
Intracellular trafficking, secretion, and vesicular transport 562194 ± 18826 554831 ± 20164 0.79
Posttranslational modification, protein turnover, chaperones 1524499 ± 49713 1432079 ± 49258 0.22
Energy production and conversion 2567778 ± 60845 2322549 ± 114626 0.09
Carbohydrate transport and metabolism 3128111 ± 70640 2698067 ± 79519 0.00
Amino acid transport and metabolism 4248646 ± 60952 3751842 ± 140894 0.01
Nucleotide transport and metabolism 1711731 ± 62403 1629905 ± 63121 0.38
Coenzyme transport and metabolism 1678606 ± 75618 1629827 ± 73324 0.65
Lipid transport and metabolism 1066536 ± 42025 1065261 ± 36048 0.98
Inorganic ion transport and metabolism 2351984 ± 102963 2298300 ± 87792 0.70
Secondary metabolites biosynthesis, transport, and catabolism 206926 ± 9555 190387 ± 8092 0.22
Function unknown 6627472 ± 327201 6695151 ± 247724 0.87
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Discussion

In the present study, a gilt obesity model was used to identify microbiota markers associated with placental oxidative stress. We found that gilts with a high backfat thickness showed a decrease in the birth weight of piglets. This result was in line with previous observation, where it was reported that maternal obesity led to a decrease in the birth weight of piglets (Zhou et al., 2018; Hu et al., 2019a). Hormone regulates fetal growth. Therefore, the levels of hormones in serum were measured. Here, no difference was observed in the concentrations of estradiol, prolactin, or FSH in the maternal serum of the two groups, while obese gilts showed a lower trend level in the serum progesterone, which was consistent with previous observation (Goh et al., 2016). Low serum progesterone was a risk factor for low birth weight (He et al., 2016), suggesting that a decreased birth weight induced by maternal obesity might attribute to the imbalance of progesterone secretion.

Placenta is the main tissue for progesterone secretion during pregnancy (López Bernal, 2007); in turn, progesterone supports placental growth and function (Mark et al., 2006). Evidences showed that maternal obesity impairs placental function (Hu et al., 2019a). In the present study, we showed that maternal obesity increased the oxidative stress levels in placenta, as evidenced by increased ROS level and the decreased SOD level, which was in line with a previous study showing that the placental ROS level was increased by maternal adiposity (Mele et al., 2014). Oxidative stress induces oxidative damage to lipid and protein through lipid and protein peroxidation (Dalle-Donne et al., 2003; Guéraud et al., 2010). A higher level of MDA and protein carbonyl in placenta further confirmed that the placenta of obese gilts was subjected to a higher oxidative stress. Mitochondria are the major ROS generation sites, and most of the ROS are generated by Complex I (Nishikawa et al., 2007; Kim and Byzova, 2014). In the present study, the activity of placental complex I was lower among obese gilts, suggesting that mitochondrial function might be functionally impaired, thus contributing to ROS generation. In addition, a decreased placental mitochondrial function was also observed among obese gilts, as evidenced by a decreased ATP level, citrate synthase activity, and the protein level of PGC-1α. In support of our view, an impaired mitochondrial function of human placentae with an increased maternal adiposity was also reported in a previous study (Mele et al., 2014). Overproduction of ROS can destroy normal placental functions (Wu et al., 2016). Therefore, we suspected that the reduction of progesterone induced by maternal obesity might be attributed to placenta dysfunction.

A previous study has showed that the intestinal microbiota played an important role in oxidative stress (Chen et al., 2020). Therefore, we firstly investigated the effects of maternal obesity on fecal microbiota composition. Our study showed that the microbial diversity was significantly decreased by obesity, as evidenced by ACE, Chao 1, and Simpson index. In addition, the Bacteroidetes and Firmicutes were the dominant phyla in feces. Firmicutes bacteria have a better capacity than Bacteroidetes bacteria in the ferment and metabolize carbohydrates as well as lipids, thus contributing to the development of obesity (Stojanov and Berlec, 2020). Gilts from Obese group displayed a higher abundance of Firmicutes and a lower abundance of Bacteroidetes, which was in line with a previous study showing that the relative proportion of Bacteroidetes was decreased among obese people in comparison with lean people (Ley et al., 2006). Consistence with the change of the abundances of Firmicutes and Bacteroidetes, the abundances of norank_f_ Bacteroidetes_S24-7_group and Alloprevotella (belonging phylum Bacteroidetes) were lower, and that of Lachnospiraceae_XPB1014_group, Ruminococcaceae_UCG-002, Streptococcus, and Christensenellaceae_R-7_group (belonging to Firmicutes) were higher in the Obese group than in the Con group. The relationship between microbiota composition and placental oxidative stress was revealed through Spearman analysis. We observed that the abundance of Christensenellaceae_R-7_group was positively correlated with the concentrations of ROS, protein carboxyl, and IL-6 in placentae, and that of norank_f:Bacteroidales_S24-7_group was negatively correlated with the levels of placental ROS, protein carboxyl, and IL-6. Changes in the intestinal microbiota was reported to induce oxidative stress. For instance, germ-free mice were infused intracolonically with fecal supernatants of acute ischemic stroke increased the levels of ROS and MDA (Xu et al., 2018); suppression of the gut microbiome ameliorates age-related arterial dysfunction and oxidative stress in mice (Brunt et al., 2019). Intestine microbiota also shapes host immune responses. Germ-free mice demonstrated that microbiota colonization in early life is necessary for development of the immune system, absence of microbiota resulted in a weakened capacity to fight off pathogenic bacteria (Sommer and Bäckhed, 2013). Therefore, we suspected that maternal obesity might induce placental oxidative damage and inflammatory response through modulating the abundance of Christensenellaceae_R-7_group and norank_f:Bacteroidales_S24-7_group. However, the mechanism needs further investigation.

SCFAs are a possible link between the intestinal microbiota and placenta (Kumar et al., 2015). Therefore, the concentration of SCFAs in feces was determined in the present study. Our data showed that the concentration of propionate was lower in Obese group than in Con group. In addition, the concentration of propionate was negatively correlated with that of protein carboxyl and IL-6 in placenta. Propionate treatment was shown to be effective against oxidative stress and ameliorate systemic inflammation (Hoyles et al., 2018; Bartolomaeus et al., 2019). Moreover, the secretion of pro-inflammatory cytokines and chemokines in placenta was blocked by a propionate treatment (Roy et al., 2020). Based on these lines of evidence available, we suspected that a decreased concentration of propionate might partially contribute to the development of placental oxidative stress. Interestingly, the concentration of propionate was positively correlated with that of serum progesterone. In line with our study, the infusion of propionate led to an increased concentration of plasma progesterone in a dairy heifer model (Bedford et al., 2018). These data indicated that a decreased propionate production might induce abnormal placental function, thus contributing to the decrease of progesterone secretion. Previous study showed that propionate and butyrate enhance mitochondrial biogenesis through extracellular signal-regulated kinases 1/2-dependent mechanism (Ribeiro et al., 2020), suggesting intestine microbiota modulate mitochondrial biogenesis thought regulating SCFAs production. Propionate is produced through the fermentation of dietary carbohydrate and amino acid by the intestinal microbiota (Neis et al., 2015). Therefore, we employed PICRUSt analysis to investigate the function of microbiota to determine the metabolic alterations caused by obesity. In the present study, microbiota in obesity gilts had a lower abundance in the transport and metabolism of carbohydrate and amino acid, indicating that a decreased carbohydrate and amino acid metabolism of microbiota might lead to the reduction of propionate production.

Conclusions

We found that maternal obesity during late pregnancy increased placental oxidative damage, induced mitochondrial dysfunction, and decreased birth weight of newborn. We identified that the microbiota markers Christensenellaceae_R-7_group and norank_f:Bacteroidales_S24-7_group were associated with placental oxidative stress. The results of the present study contribute to the first evidence that the intestinal microbiota is an important mediator of obesity‐related placental oxidative stress and suggest that therapeutic strategies targeted at intestinal microbiota health may preserve placental function and reduce the risk of pregnancy syndromes in humans.

Data Availability Statement

The datasets presented in this study can be found in online repositories. The names of the repository/repositories and accession number(s) can be found below: NCBI SRA [accession: SRR14292254–SRR14292265].

Ethics Statement

This study was performed in accordance with the recommendations of the Guide for the Care and Use of Chinese Academy of Tropical Agricultural Sciences.

Author Contributions

CH, YY and HZ contributed to the study design, conducted the animal experiments, and wrote the manuscript. CH and YY executed the lab analysis. YY and FJ performed the statistical analysis and HZ revised the paper. All authors contributed to the article and approved the submitted version.

Funding

The present work was jointly supported by Central Public-interest Scientific Institution Basal Research Fund for Chinese Academy of Tropical Agricultural Sciences (No.1630032021004) and the Integrated Demonstration of Key Techniques for the Industrial Development of Featured Crops in Rocky Desertification Areasof Yunnan-Guangxi-Guizhou Provinces (SMH2019-2021).

Conflict of Interest

The authors declare that the research was conducted in the absence of any commercial or financial relationships that could be construed as a potential conflict of interest.

Publisher’s Note

All claims expressed in this article are solely those of the authors and do not necessarily represent those of their affiliated organizations, or those of the publisher, the editors and the reviewers. Any product that may be evaluated in this article, or claim that may be made by its manufacturer, is not guaranteed or endorsed by the publisher.

Supplementary Material

The Supplementary Material for this article can be found online at: https://www.frontiersin.org/articles/10.3389/fcimb.2021.671347/full#supplementary-material

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References

  1. Bartolomaeus H., Balogh A., Yakoub M., Homann S., Markó L., Höges S., et al. (2019). Short-Chain Fatty Acid Propionate Protects From Hypertensive Cardiovascular Damage. Circulation 139, 1407–1421.   10.1161/CIRCULATIONAHA.118.036652 [DOI] [PMC free article] [PubMed] [Google Scholar]
  2. Bedford A., Beckett L., Hardin K., Dias N. W., Davis T., Mercadante V. R. G., et al. (2018). Propionate Affects Insulin Signaling and Progesterone Profiles in Dairy Heifers. Sci. Rep. 8, 17629.   10.1038/s41598-018-35977-1 [DOI] [PMC free article] [PubMed] [Google Scholar]
  3. Brunt V. E., Gioscia-Ryan R. A., Richey J. J., Zigler M. C., Cuevas L. M., Gonzalez A., et al. (2019). Suppression of the Gut Microbiome Ameliorates Age-Related Arterial Dysfunction and Oxidative Stress in Mice. J. Physiol. 597, 2361–2378.   10.1113/JP277336 [DOI] [PMC free article] [PubMed] [Google Scholar]
  4. Chen X., Li P., Liu M., Zheng H., He Y., Chen M. X., et al. (2020). Gut Dysbiosis Induces the Development of Pre-Eclampsia Through Bacterial Translocation. Gut 69, 513–522.   10.1136/gutjnl-2019-319101 [DOI] [PubMed] [Google Scholar]
  5. Dalle-Donne I., Rossi R., Giustarini D., Milzani A., Colombo R. (2003). Protein Carbonyl Groups as Biomarkers of Oxidative Stress. Clin. Chim. Acta 329, 23–38.   10.1016/s0009-8981(03)00003-2 [DOI] [PubMed] [Google Scholar]
  6. Godfrey K. M., Reynolds R. M., Prescott S. L., Nyirenda M., Jaddoe V. W., Eriksson J. G., et al. (2017). Influence of Maternal Obesity on the Long-Term Health of Offspring. Lancet Diabetes Endocrinol. 5, 53–64.   10.1016/S2213-8587(16)30107-3 [DOI] [PMC free article] [PubMed] [Google Scholar]
  7. Goh J. Y., He S., Allen J. C., Malhotra R., Tan T. C. (2016). Maternal Obesity Is Associated With a Low Serum Progesterone Level in Early Pregnancy. Horm. Mol. Biol. Clin. Investig. 27, 97–100.   10.1515/hmbci-2015-0030 [DOI] [PubMed] [Google Scholar]
  8. Guéraud F., Atalay M., Bresgen N., Cipak A., Eckl P. M., Huc L., et al. (2010). Chemistry and Biochemistry of Lipid Peroxidation Products. Free Radic. Res. 44, 1098–1124.   10.3109/10715762.2010.498477 [DOI] [PubMed] [Google Scholar]
  9. He S., Allen J. C., Jr., Malhotra R., Østbye T., Tan T. C. (2016). Association of Maternal Serum Progesterone in Early Pregnancy With Low Birth Weight and Other Adverse Pregnancy Outcomes. J. Matern Fetal Neonatal Med. 29, 1999–2004.   10.3109/14767058.2015.1072159 [DOI] [PubMed] [Google Scholar]
  10. Hoyles L., Snelling T., Umlai U. K., Nicholson J. K., Carding S. R., Glen R. C., et al. (2018). Microbiome-Host Systems Interactions: Protective Effects of Propionate Upon the Blood-Brain Barrier. Microbiome 6, 55.   10.1186/s40168-018-0439-y [DOI] [PMC free article] [PubMed] [Google Scholar]
  11. Hu C., Li F., Duan Y., Yin Y., Kong X. (2019. b). Dietary Supplementation With Leucine or in Combination With Arginine Decreases Body Fat Weight and Alters Gut Microbiota Composition in Finishing Pigs. Front. Microbiol. 10, 1767.   10.3389/fmicb.2019.01767 [DOI] [PMC free article] [PubMed] [Google Scholar]
  12. Hu C., Li F., Duan Y., Yin Y., Kong X. (2019. c). Glutamic Acid Supplementation Reduces Body Fat Weight in Finishing Pigs When Provided Solely or in Combination With Arginine and It Is Associated With Colonic Propionate and Butyrate Concentrations. Food Funct. 10, 4693–4704.   10.1039/c9fo00520j [DOI] [PubMed] [Google Scholar]
  13. Hu C., Yang Y., Li J., Wang H., Cheng C., Yang L., et al. (2019. a). Maternal Diet-Induced Obesity Compromises Oxidative Stress Status and Angiogenesis in the Porcine Placenta by Upregulating Nox2 Expression. Oxid. Med. Cell Longev 2019, 2481592.   10.1155/2019/2481592 [DOI] [PMC free article] [PubMed] [Google Scholar]
  14. Kim Y. W., Byzova T. V. (2014). Oxidative Stress in Angiogenesis and Vascular Disease. Blood 123, 625–631.   10.1182/blood-2013-09-512749 [DOI] [PMC free article] [PubMed] [Google Scholar]
  15. Kumar P., Thirkill T. L., Ji J., Monte L. H., Douglas G. C. (2015). Differential Effects of Sodium Butyrate and Lithium Chloride on Rhesus Monkey Trophoblast Differentiation. PloS One 10, e0135089.   10.1371/journal.pone.0135089 [DOI] [PMC free article] [PubMed] [Google Scholar]
  16. Ley R. E., Turnbaugh P. J., Klein S., Gordon J. I. (2006). Microbial Ecology: Human Gut Microbes Associated With Obesity. Nature 444, 1022–1023.   10.1038/4441022a [DOI] [PubMed] [Google Scholar]
  17. López Bernal A. (2007). Overview. Preterm Labour: Mechanisms and Management. BMC Pregnancy Childbirth 7 (Suppl 1), S2.   10.1186/1471-2393-7-S1-S2 [DOI] [PMC free article] [PubMed] [Google Scholar]
  18. Mark P. J., Smith J. T., Waddell B. J. (2006). Placental and Fetal Growth Retardation Following Partial Progesterone Withdrawal in Rat Pregnancy. Placenta 27, 208–214.   10.1016/j.placenta.2005.01.004 [DOI] [PubMed] [Google Scholar]
  19. Mele J., Muralimanoharan S., Maloyan A., Myatt L. (2014). Impaired Mitochondrial Function in Human Placenta With Increased Maternal Adiposity. Am. J. Physiol. Endocrinol. Metab. 307, E419–E425.   10.1152/ajpendo.00025.2014 [DOI] [PMC free article] [PubMed] [Google Scholar]
  20. Myatt L., Maloyan A. (2016). Obesity and Placental Function. Semin. Reprod. Med. 34, 42–49.   10.1055/s-0035-1570027 [DOI] [PubMed] [Google Scholar]
  21. Neis E. P., Dejong C. H., Rensen S. S. (2015). The Role of Microbial Amino Acid Metabolism in Host Metabolism. Nutrients 7, 2930–2946.   10.3390/nu7042930 [DOI] [PMC free article] [PubMed] [Google Scholar]
  22. Ng M., Fleming T., Robinson M., Thomson B., Graetz N., Margono C., et al. (2014). Global, Regional, and National Prevalence of Overweight and Obesity in Children and Adults During 1980-2013: A Systematic Analysis for the Global Burden of Disease Study 2013. Lancet 384, 766–781.   10.1016/S0140-6736(14)60460-8 [DOI] [PMC free article] [PubMed] [Google Scholar]
  23. Nishikawa T., Kukidome D., Sonoda K., Fujisawa K., Matsuhisa T., Motoshima H., et al. (2007). Impact of Mitochondrial ROS Production on Diabetic Vascular Complications. Diabetes Res. Clin. Pract. Suppl 1, S41–S45.   10.1016/j.diabres.2007.01.031 [DOI] [PubMed] [Google Scholar]
  24. Ribeiro M. F., Santos A. A., Afonso M. B., Rodrigues P. M., Sónia S. S., m Castro R. E., et al. (2020). Diet-Dependent Gut Microbiota Impacts on Adult Neurogenesis Through Mitochondrial Stress Modulation. Brain Commu 2, fcaa165.   10.1093/braincomms/fcaa165 [DOI] [PMC free article] [PubMed] [Google Scholar]
  25. Roy R., Nguyen-Ngo C., Lappas M. (2020). Short-Chain Fatty Acids as Novel Therapeutics for Gestational Diabetes. J. Mol. Endocrinol. 65, 21–34.   10.1530/JME-20-0094 [DOI] [PubMed] [Google Scholar]
  26. Sommer F., Bäckhed F. (2013). The Gut Microbiota - Masters of Host Development and Physiology. Nat. Rev. Microbiol. 11, 227–238.   10.1038/nrmicro2974 [DOI] [PubMed] [Google Scholar]
  27. Song T., Lu J., Deng Z., Xu T., Yang Y., Wei H., et al. (2018). Maternal Obesity Aggravates the Abnormality of Porcine Placenta by Increasing N(6)-Methyladenosine. Int. J. Obes. 42, 1812–1820.   10.1038/s41366-018-0113-2 [DOI] [PubMed] [Google Scholar]
  28. Stojanov S., Berlec A. (2020). The Influence of Probiotics on the Firmicutes/Bacteroidetes Ratio in the Treatment of Obesity and Inflammatory Bowel Disease. Microorganisms 8, 1715.   10.3390/microorganisms8111715 [DOI] [PMC free article] [PubMed] [Google Scholar]
  29. Tauqeer Z., Gomez G., Stanford F. C. (2018). Obesity in Women: Insights for the Clinician. J. Womens Health 27, 444–457.   10.1089/jwh.2016.6196 [DOI] [PMC free article] [PubMed] [Google Scholar]
  30. Wang H., Hu C., Cheng C., Cui J., Ji Y., Hao X., et al. (2019). Unraveling the Association of Fecal Microbiota and Oxidative Stress With Stillbirth Rate of Sows. Theriogenology 136, 131–137.   10.1016/j.theriogenology.2019.06.028 [DOI] [PubMed] [Google Scholar]
  31. Wu F., Tian F. J., Lin Y., Xu W. M. (2016). Oxidative Stress: Placenta Function and Dysfunction. Am. J. Reprod. Immunol. 76, 258–271.   10.1111/aji.12454 [DOI] [PubMed] [Google Scholar]
  32. Xu N., Kan P., Yao X., Yang P., Wang J., Xiang L., et al. (2018). Astragaloside Iv Reversed the Autophagy and Oxidative Stress Induced by the Intestinal Microbiota of Ais in Mice. J. Microbiol. 56, 838–846.   10.1007/s12275-018-8327-5 [DOI] [PubMed] [Google Scholar]
  33. Zhang Y., Sowers J. R., Ren J. (2018). Targeting Autophagy in Obesity: From Pathophysiology to Management. Nat. Rev. Endocrinol. 14, 356–376.   10.1038/s41574-018-0009-1 [DOI] [PubMed] [Google Scholar]
  34. Zhi C., Huang J., Wang J., Cao H., Bai Y., Guo J., et al. (2019). Connection Between Gut Microbiome and the Development of Obesity. Eur. J. Clin. Microbiol. Infect. Dis. 38, 1987–1998.   10.1007/s10096-019-03623-x [DOI] [PubMed] [Google Scholar]
  35. Zhou Y., Xu T., Cai A., Wu Y., Wei H., Jiang S., et al. (2018). Excessive Backfat of Sows at 109 D of Gestation Induces Lipotoxic Placental Environment and Is Associated With Declining Reproductive Performance. J. Anim. Sci. 96, 250–257.   10.1093/jas/skx041 [DOI] [PMC free article] [PubMed] [Google Scholar]

Associated Data

This section collects any data citations, data availability statements, or supplementary materials included in this article.

Supplementary Materials

Click here for additional data file. (244.4KB, docx)

Data Availability Statement

The datasets presented in this study can be found in online repositories. The names of the repository/repositories and accession number(s) can be found below: NCBI SRA [accession: SRR14292254–SRR14292265].

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