Skip to main content
Download PDF

Dysfunction of DMT1 and miR-135b in the gut-testis axis in high-fat diet male mice

Genes & Nutrition volume 19, Article number: 1 (2024) Cite this article

Abstract

Background

Obese patients have been found to be susceptible to iron deficiency, and malabsorption of dietary iron is the cause of obesity-related iron deficiency (ORID). Divalent metal transporter 1 (DMT1) and ferroportin (FPN), are two transmembrane transporter proteins expressed in the duodenum that are closely associated with iron absorption. However, there have been few studies on the association between these two proteins and the increased susceptibility to iron deficiency in obese patients. Chronic inflammation is also thought to be a cause of obesity-related iron deficiency, and both conditions can have an impact on spermatogenesis and impair male reproductive function. Based on previous studies, transgenerational epigenetic inheritance through gametes was observed in obesity.

Results

Our results  showed that obese mice had decreased blood iron levels (p < 0.01), lower protein and mRNA expression for duodenal DMT1 (p < 0.05), but no statistically significant variation in mRNA expression for duodenal FPN (p > 0.05); there was an increase in sperm miR-135b expression (p < 0.05). Bioinformatics revealed ninety overlapping genes and further analysis showed that they were primarily responsible for epithelial cilium movement, fatty acid beta-oxidation, protein dephosphorylation, fertilization, and glutamine transport, which are closely related to spermatogenesis, sperm development, and sperm viability in mice.

Conclusions

In obese mice, we observed downregulation of DMT1 in the duodenum and upregulation of miR-135b in the spermatozoa.

Background

Obesity has become a global epidemic that endangers human health and increases the medical burden on society. Body mass index (BMI) is used to estimate a person’s weight category (normal/overweight/obese), and in 2016, 39% of individuals above the age of 17 were considered to be overweight (BMI ≥ 25), while 13% were obese (BMI ≥ 30) [1]. Current data suggest that by 2038, over one-third of the global population will be obese [2]. According to a 1961 study by Wenzel et al. [3], obese individuals had lower serum iron concentrations than non-obese persons and this has subsequently been supported by the findings of other researchers [4]. There has been an increase in studies showing that obesity affects micronutrient absorption, especially iron, which can lead to iron deficiency or even iron deficiency anemia [5,6,7]. Dietary absorption of stable isotope tracer iron was significantly lower in obese children than in non-obese control children [8], suggesting that dietary iron malabsorption could be an important cause of obesity-related iron deficiency.

Iron is an essential trace element for the human body and an essential biological element for almost all organisms, as it is involved in such biological processes as transport and storage of oxygen and electron transfer. Iron deficiency can lead to immune system disorders, and anemia, and even affect growth and motor development in children [9]. The duodenum is one of the main sites of iron absorption and is critical for the regulation of iron homeostasis [10]. Iron in food is mainly in the form of Fe3+, which is reduced to Fe2+ by duodenal cytochrome b (Dcytb) located on the duodenal parietal membrane. DMT1, a transmembrane transporter protein on the duodenal parietal membrane, then transports Fe2+ into the cell [11,12,13,14]. Iron entering small intestinal cells is released after passing through another transmembrane transporter protein, FPN, which is the only known channel protein for the extracellular transport of non-heme iron and plays an important role in development and intestinal iron absorption in mice [15].

Obesity is characterized by an excessive accumulation of fatty adipose tissue. Immune cells such as macrophages and lymphocytes in adipose tissue can be activated and release inflammatory factors like TNF-α, leading to chronic inflammation [16]. Chronic inflammation is also associated with anemia and is one of the reasons why obese patients are prone to iron deficiency [17]. Hepcidin is a small peptide secreted by the liver that inhibits intestinal iron absorption and helps to regulate iron homeostasis. Chronic inflammation produces the pro-inflammatory cytokine, interleukin-6 (IL-6), which induces the production of hepatic hepcidin. Therefore, some investigators have suggested that inflammation-induced upregulation of hepcidin expression may be a potential modulator between obesity and iron deficiency [18,19,20,21,22]. Pro-inflammatory cytokines may also affect erythropoietin levels and increase iron retention by reticuloendothelial cells, leading to anemia in some obese individuals [23]. ORID and abnormal iron absorption have many adverse effects on the male reproductive system. Iron deficiency can impair sperm development and increase oxidative damage to sperm [24] as well as reduce ejaculate volume, sperm count, and sperm viability [25, 26]. Studies have shown that although serum iron is lower in obese people, iron levels in seminal plasma and spermatozoa are high [27]; however, higher iron levels in seminal plasma are negatively associated with male fertility, and the adverse effects may be mediated by oxidative stress [28].

RNA is one of the epigenetic markers of germ cells, and phenotypic changes resulting from exposure of the father to certain environmental factors can be inherited by the offspring through sperm RNAs. For example, western diet-induced phenotypic inheritance can be mediated through sperm RNAs [29]. Small non-coding RNAs (sncRNAs) can transmit information about environmental factors and are carriers of environmental influences to the genome [30]. These sncRNAs are abundant in sperm and play an important role in cross-generational inheritance [31]. MicroRNAs (miRNAs) are a group of sncRNAs 20–23 nucleotides in length encoded by the genome, which directs the RNA-induced silencing complex (RISC) to degrade mRNAs or block their translation by base-pairing with target gene mRNAs. There are many miRNAs such as miR-135b that have been shown to be closely associated with inflammation, and interleukin 1 can upregulate miR-135b expression to promote inflammation [32].

To investigate whether the ORID is associated with duodenal DMT1 and FPN expression, we used a high-fat diet-induced obese mouse model. The serum iron levels of the obese mice were determined and the expression levels of duodenal DMT1 and FPN were assessed by immunohistochemical methods and quantitative real-time polymerase chain reaction (qRT-PCR). The expression of sperm miR-135b in obese mice was also measured by qRT-PCR, and the data were subjected to bioinformatics analysis. Consistent with human data, we confirmed that serum iron levels were also lower in obese mice and that lower DMT1 mRNA and protein levels could inhibit duodenal iron absorption. Due to its positive correlation with inflammation, the high expression of miR-135b in the sperm of obese mice suggested that the sperm were indeed affected by inflammation. Further bioinformatics analysis revealed that miR-135b affected fertility in obese mice, including spermatogenesis, sperm development, and fertilization.

Materials and methods

Animal experiments and a mouse model of obesity

The animal protocols and care were in accordance with the guidelines of Xi'an Jiaotong University’s Animal Experimental Ethics Committee. The animals used in the experiments were provided by the Xi’an Jiaotong University Health Science Center. Twenty male-specific pathogen-free (SPF) ICR mice (5 weeks old) were used in this study. After 1 week of acclimatization, the mice were randomly separated into two groups of ten each. The control group was fed the standard diet (SD) that provided 10% fat energy (DIO12450B, Beijing Keao Xieli Feed Co., Ltd). The model group received a high-fat diet (HFD) containing a 60% fat-energy ratio chow (DIO12492, Beijing Keao Xieli Feed Co., Ltd.). The mice were fed for nine weeks and their body weight was measured once a week. The temperature and humidity were controlled, and the mice were kept on a 12-h light/12-h dark cycle each day.

Collection of blood and other samples

After feeding, mice were fasted for 6 h, anesthetized using tribromoethanol (M2920, Jiangsu Yihe Scientific Instrument Co., China), and then blood was drawn. Subsequently, the mice were euthanized by cervical dislocation, after which their duodenum, testes, and bilateral epididymal tails were immediately removed. After standing for 30 min, the blood was centrifuged at 1800 × g, the supernatants were collected into fresh tubes, centrifuged a second time at 1800 × g for 5 min, and the supernatants were collected again after centrifugation to obtain the serum. For sperm collection, the epididymal tails were clipped and placed in 1.5 ml of PBS (130 mM NaCl, 10 mM Na2PO4, 1.7 mM KH2PO4, 2 mM KCl, pH 7.4) and kept at 37 °C for 15 min to allow sperm release. The suspension was filtered through a 40-μm cell filter to remove tissue pieces, and the filtrate was mixed with 10 volumes of somatic cell lysis solution (0.1% SDS, 0.5% Triton X-100, DEPC H2O), and kept on ice for 40 min after mixing for 5 min. A visible light microscope was used to confirm that the somatic cells were all lysed. The suspension was centrifuged at 10,000 × g for 8 min at 4 °C, and the sperm pellet was washed twice with PBS and again centrifuged under the same conditions. The supernatant was removed and TRIzol reagent was added for RNA extraction. After duodenal samples were collected, one part was placed into nuclease-free tubes with TRIzol reagent for RNA extraction, and the other part and the testes were placed in 4% paraformaldehyde and fixed at room temperature for 24 h.

Serum iron assay

Serum iron content was determined using a serum iron assay kit (A039-1–1, Nanjing Jiancheng Bioengineering Institute, China), following kit instructions. The absorbance was detected at 520 nm with a microplate spectrophotometer.

Hematoxylin and Eosin (H&E) and immunohistochemistry staining

After fixation, the duodenum and the testes samples were rinsed with running water for 30 min, then dehydrated in graded ethanol and cleared. After being embedded in paraffin, samples were sliced into 5-μm sections, dewaxed with xylene for 10 min, and rinsed in 100%, 95%, and 90% ethanol for 3 min.

For HE staining, the sections were dehydrated after staining with HE reagent and then sealed with a neutral fixative. For immunohistochemistry staining, sodium citrate antigen epitope retrieval solution (MVS-0101, Fuzhou Maixin Biotech, China) was used for antigen retrieval by heating in a microwave. The sections were next blocked with 10% goat serum (AR0009, Boster Biological Technology, China) at 37 °C for 30 min. This treatment reduces the non-specific binding of the subsequent primary and secondary antibodies to the samples and lowers the background. Primary antibody immunostaining solution (P0262, Shanghai Biyuntian Biotechnology, China) was used to dilute the DMT1 antibody (A10231, ABclonal Technology, China) at a ratio of 1:200, and sections were transferred to wet boxes for overnight incubation with primary antibody at 4 °C. Sections were rinsed three times with PBS. Immunostaining secondary Ab diluent (P0265, Shanghai Biyuntian Biotechnology, China) was used to dilute HRP-conjugated goat anti-rabbit IgG H&L at a ratio of 1:200. After adding secondary Ab, the sections were transferred to the wet box for 1 h at 37 ℃, then rinsed with PBS. Sections were stained with DAB for 5 s and then with hematoxylin for the nucleus. After rinsing, the sections were dehydrated, covered with neutral fixative, digitally imaged under a visible light microscope, and analyzed.

RNA extraction and qRT-PCR

RNA was extracted from duodenal and sperm samples using the TRIzol method, and RNA concentrations and A260/A280 were measured using a UV spectrophotometer. Complementary DNA (cDNA) was synthesized from 1 μg of total duodenal RNA using the Evo M-MLV RT mix kit with gDNA-Clean for qPCR (AG11728, Accurate Biology, China). The miRNA 1st strand cDNA synthesis kit (stem-loop) (AG11743, Accurate Biology, China) was employed to synthesize cDNA from 200 ng of gross sperm RNA from sperm samples. SYBR® Green Premix Pro Taq HS qPCR kit (AG11701, Accurate Biology, China) was used to measure mRNA expression levels in a 20-μL total reaction system. Glyceraldehyde-3-phosphate dehydrogenase (GAPDH) was used as the internal normalization control for duodenal RNA and U6 as the internal normalization control for sperm RNA. Table 1 lists the qRT-PCR primer sequences, which were synthesized by the Tsingke Biotechnology Co. (https://tsingke.com.cn/).

Table 1 Primers used for gene expression assay by RT-qPCR
Full size table

MiRNA target gene prediction and functional annotation

The miRWalk online tool (http://mirwalk.umm.uni-heidelberg.de/) was used to predict the target genes of miR-135b. Relevant keywords were entered in the National Center of Biotechnology Information (NCBI) Gene Expression Omnibus (GEO; http://0-www-ncbi-nlm-nih-gov.brum.beds.ac.uk/geo/) database, and the GSE133915 dataset was identified and downloaded. The mRNA expression database included 16 samples, eight sperm samples for the HFD group and eight sperm samples for the SD group. The Xiantao Academic online tool (https://www.xiantaozi.com/) was used for the DESeq2 analysis. The DESeq2 package was used to perform differential expression analysis on the original counts matrix, following the standard procedure, and the variance stabilizing transformations (VST) method provided by the DESeq2 package was used to normalize the original counts matrix. The screening conditions were |log2 (fold-change) |> 0.58 and p < 0.05, and 2149 differentially expressed genes (DEGs) were screened. The Venn diagram online mapping tool (http://bioinformatics.psb.ugent.be/webtools/Venn/) was used to indicate the overlaps of DEGs and predicted target genes. The database for annotation, visualization and integrated discovery (DAVID) (https://david.ncifcrf.gov/) was used for gene ontology (GO) and the Kyoto Encyclopedia of Genes and Genomes (KEGG) for pathway analysis of overlapping genes. Mouse genome informatics (MGI) (https://www.informatics.jax.org/) was used to search all genes related to the male sterile phenotype in mice and the gene ontology (GO) knowledgebase (http://geneontology.org/) was used to search for genes associated with fertilization, sperm development and spermatogenesis in mice.

Statistical analysis

The image intensity of the duodenal DMT1 staining results was determined using Image-Pro Plus 6.0, 10 randomly chosen, 200 × fields per section were evaluated for each mouse. Data are mean ± standard error of the mean (SEM). SPSS was employed to analyze serum iron levels, DMT1, and FPN expression in the duodenum, and data were compared using Student’s t test. A value of p < 0.05 was regarded as significantly different in statistical terms.

Results

Abnormal testes morphology in obese mice

To establish the HFD-induced obesity model in mice, we divided the mice into two groups, SD and HFD, with feeding of 10% and 60% fat energy ratio, respectively. Initially, the mean body weights of mice were 23.8 g ± 0.95 in the HFD and 23.2 g ± 1.32 in the SD group. By the end of 9 weeks, the mean body weights of the mice in the HFD and SD groups were 42.38 g ± 2.18 and 32.08 g ± 1.38, respectively, and the body weights of the HFD mice exceeded the mean body weights of the SD mice by 20%.

In our study, HE staining was performed on testicular sections from both obese mice and the control group to evaluate the potential impact of obesity on male reproductive function (Fig. 1A). In the SD control group, seminiferous tubules exhibited clear identification of spermatogonia, spermatocytes at various stages, and spermatozoa. In contrast, the HFD group displayed sparser cellular arrangement within the seminiferous tubules, reduced number of spermatogonia, thinning of the germinal epithelium, and a notable absence of spermatozoa in most tubules. In conclusion, the HE-stained testicular sections from the HFD group demonstrated several morphological abnormalities compared to the SD control group, suggesting that obesity adversely affects male reproductive function in mice.

Fig. 1
figure 1

Effects of HFD on testicular morphology and serum iron levels. A Morphological analysis of testis from SD and HFD groups. B Serum iron levels were significantly decreased in HFD-fed obese mice compared to SD-fed control mice. Data are expressed as mean ± SEM; **p < 0.01

Full size image

Serum iron

The serum iron levels in both groups of mice were measured, and the results showed that the serum iron levels were significantly lower in the obese mice compared with the SD control (Fig. 1B).

Expression levels of duodenal DMT1 and FPN

To evaluate the impact of obesity on duodenal iron absorption, we determined the expression levels of duodenal DMT1 in the two groups of mice by immunohistochemistry and qRT-PCR. The DMT1 protein and mRNA levels were significantly decreased in the duodenum of HFD-induced obese mice compared to normal weight controls (Fig. 2A, B). The expression levels of FPN in the duodenum were also compared by qRT-PCR, which showed no difference in FPN mRNA expression in the duodenum (Fig. 2C).

Fig. 2
figure 2

HFD-induced obesity reduces the protein and mRNA expression of duodenal DMT1. A Immunohistochemical staining of duodenal DMT1 in SD and HFD mice. The mRNA expression levels of B DMT1 and C FPN in SD and HFD mice. Data are expressed as SEM ± mean; *p < 0.05; ns indicates p > 0.05

Full size image

Expression of miR-135b in sperm and functional annotation of DEGs

The qRT-PCR method was performed to evaluate miR-135b expression in the spermatozoa of obese mice compared to normal-weight mice. The results (Fig. 3A) showed that the expression level of miR-135b was significantly increased in the spermatozoa of mice on the HFD compared with those fed the SD.

Fig. 3
figure 3

Expression of miR-135b in sperm and functional annotation of DEGs. A Expression of miR-135b from sperm of SD vs HFD mice; *p < 0.05. B Bubble diagram of GO for 90 DEGs. Venn diagrams of 90 DEGs and genes related to C male sterility phenotype, D fertilization, E spermatogenesis, and F spermatozoa development

Full size image

GSE133915 is the set of transcriptome data comparing the spermatozoa of mice in the SD group and HFD group by RNA sequencing. The Xiantao Academic online tool was used to perform DESeq2 analysis on the transcriptome data with a screening condition of |log2 (fold-change) |> 0.58 and p < 0.05. A total of 2149 DEGs were screened, of which 1924 genes were upregulated and 225 genes were downregulated. Target genes of miR-135b were predicted using the miRWalk platform. Overlapping genes of target genes and DEGs were shown as Venn diagrams using an online mapping tool, and a total of 90 genes were obtained, of which 79 were upregulated and 11 were downregulated. GO analysis (Fig. 3B) was used to determine the biological process (BP), molecular function (MF), and cellular component (CC) classifications of these 90 genes, and p < 0.05 was considered significantly enriched. The top 12 BPs were enriched in phosphatidic acid biosynthesis, epithelial cilium movement, fatty acid beta-oxidation using acyl-CoA oxidase, protein dephosphorylation, positive regulation of actin nucleation, amino acid transport, phosphatidic acid metabolism, dorsal spinal cord development, fertilization, glutamine transport, arginine transmembrane transport, and peristalsis. The CCs were enriched in spermatid manchettes, cytoplasm, Schaffer collateral-CA1 synapses, acrosomal vesicles, cilia, retromer complexes, and microtubule-associated complexes. The MFs were enriched in protein binding, amino acid transmembrane transporter activity, protein tyrosine phosphatase activity, acyl-CoA oxidase activity, phosphoprotein phosphatase activity, L-glutamine transmembrane transporter activity, L-arginine transmembrane transporter activity, peroxisome proliferator-activated receptor binding, hydrolase activity, and metal ion binding. Within these three elements, ninety DEGs were involved in fertilization and strongly associated with spermatogenesis, sperm development, and sperm viability. KEGG enrichment had no results.

The MGI database was used to search for genes related to the mouse male sterility phenotype, and the GO knowledge base was used to search for genes related to fertilization, sperm development, and spermatogenesis in mice. Overlaps among these genes and the 90 DEGs were obtained and depicted as Venn diagrams using an online mapping tool. There were 1334 genes related to male sterility phenotype in mice, and 8 genes overlapped with the 90 DEGs (Fig. 3C), namely Spag17, Tdrd12, Stk36, Nxf2, Bard1, Lpin1, Spef2 and Jag2. There were 210 genes related to mouse fertilization and 3 genes overlapping with the 90 DEGs (Fig. 3D), namely Tdrd12, Spesp1, and Fam170b. There were 707 genes related to mouse spermatogenesis and 6 genes overlapping with the 90 DEGs (Fig. 3E), namely Ica1l, Spag17, Lztfl1, Tdrd12, Spef2, and Jag2. There were 281 genes associated with mouse spermatogenesis, and we found 5 genes overlapping with the 90 DEGs (Fig. 3F), namely Ica1l, Spesp1, Adam30, Spag17, and Spef2.

Discussion

Many previous studies have demonstrated that obese people are prone to iron deficiency, but the specific pathophysiological mechanism of this phenomenon remains incomplete. Some researchers have suggested that it is due to the intake of nutritionally unbalanced foods by obese patients. They tend to eat high-fat, high-calorie, low-nutrient foods, which can cause unbalanced intake of nutrients, including insufficient uptake of iron, thus aggravating the problem of iron deficiency. In addition, obese patients have thicker subcutaneous fat, which expands the capillary beds and leads to increased blood volume, which can also result in iron deficiency [33]. Systemic chronic inflammation is a factor of interest to a wide range of researchers, and it can decrease iron absorption by increasing the levels of hepcidin [34]. Iron homeostasis was improved in obese patients undergoing bariatric surgery, and they had significantly lower concentrations of C-reactive protein (CRP) and iron-regulated hormone in comparison to previous concentrations, presumably due to a reduction in the inflammation that may have been hindering iron absorption [35].

The duodenum is one of the major sites of iron absorption. DMT1 expressed in the duodenum is one of the key transporter proteins involved in iron uptake and the expression of duodenal DMT1 is reduced when the concentration of hepcidin is too high. At the same time, iron absorption at the tip of the intestine is inhibited, but the expression level of FPN is not altered [36, 37]. We found lower protein and mRNA expression levels of duodenal DMT1 in obese mice, but no statistically significant difference in mRNA expression of duodenal FPN between the two groups. This alteration may be due to chronic inflammation caused by obesity that increases hepcidin levels, which leads to decreased expression of duodenal DMT1, while FPN expression is not affected. Four AAs, Asp, Gln, Glu, and Gly, can increase iron absorption by increasing DMT1 expression [38], suggesting that in addition to bariatric surgery, we may also be able to prevent ORID through pharmacological interventions. In addition, we observed that HFD can also lead to morphological damage in the duodenal villi, resulting in an increased subepithelial space at the tips of some villi. This may also serve as one of the contributing factors affecting iron absorption.

Obesity, inflammation, and iron deficiency are closely related [34]. Inflammation and iron deficiency are important causes of impaired reproductive function in obese men [39,40,41]. Inflammation reduces the number of Leydig cells and spermatozoa, decreases sperm viability, and affects the synthesis of testicular steroid hormones [42, 43]. In addition to altering the microbiota, iron deficiency interferes with the expression of genes involved in spermatogenic activity, resulting in the impairment of male reproductive function [44]. Iron deficiency also increases oxidative stress in the testes, and iron supplementation can mitigate oxidative damage and repair testicular dysfunction [45].

MiR-135b expression has previously been found to be higher in the sperm of obese subjects [46], and it is strongly associated with both inflammation and embryonic development. Previously, researchers found that sperm from obese patients had higher numbers of miRNAs associated with both inflammation and iron metabolism. We found higher miR-135b expression in the spermatozoa of obese mice and performed bioinformatics analyses. The results of GO analysis showed that miR-135b affected reproductive function in obese male mice.

Cilia are organelles present on the cell surface, and the movement of epithelial cell cilia is involved in the movement of extracellular fluids, such as the transport of mucus in the respiratory tract. In males, motile cilia ensure that sperm can be smoothly transported from the testis to the epididymis for further functional maturation [47]. Fatty acid metabolism plays a very important role in sperm energy production, and fatty acid β-oxidation is an important source of energy during sperm maturation. Solute carrier family 22 member 14 (SLC22A14) regulates long-chain fatty acid β-oxidation and thus maintains energy homeostasis within spermatozoa; mutations in this gene can lead to male infertility disorders [48]. Protein phosphorylation and dephosphorylation are among the primary molecular mechanisms of sperm signaling and regulatory expression of enzymes and are also linked to sperm and egg cell signal recognition and completion of fertilization [49]. In addition, sperm capacitation cannot be achieved without tyrosine phosphorylation [50]. Sperm-egg cell fusion is one of the main processes of fertilization, and the movement of the male pronucleus to the female pronucleus of the oocyte, a process known as inward movement, is dependent on actin nucleation, which is one of the mechanisms of pronucleus migration of fertilized mouse eggs [51]. It has been shown that β-alanine, a taurine transport inhibitor, decreased reproductive hormone levels, significantly reduced sperm motility, and increased the incidence of abnormal sperm [52]. Phosphatidic acid (PA), a common phospholipid and a component of cell membranes, plays a very important role in the later stages of spermatogenesis, and phosphatidic acid levels have been associated with male infertility [53]. Glutamine and L-arginine have been proven to reduce sperm motility [54,55,56]. Thus, miR135b mainly affects sperm function in obese mice, including but not limited to sperm motility, sperm capacitation, sperm count, and fertilization.

We explained the cause of iron deficiency due to dietary obesity and revealed the role of iron deficiency and inflammation in the regulation of reproductive disorders.

Conclusion

We found lower protein and mRNA expression levels of duodenal DMT1 in obese mice, and higher miR-135b expression in the spermatozoa of obese mice. In conclusion, we demonstrated that the dyfunction of DMT1 and miR-135b in the gut-testis axis induced by HFD might be an important target impairing male fertility.

Availability of data and materials

All data generated or analyzed during this study are included in this published article.

References

  1. NCD Risk Factor Collaboration (NCD-RisC). Worldwide trends in body-mass index, underweight, overweight, and obesity from 1975 to 2016: a pooled analysis of 2416 population-based measurement studies in 128·9 million children, adolescents, and adults. Lancet. 2017;390(10113):2627–42. https://0-doi-org.brum.beds.ac.uk/10.1016/S0140-6736(17)32129-3.

    Article  Google Scholar 

  2. Lemay A, Labrie F. Electrophoretic analysis of polypeptides of plasma membranes from bovine pituitary gland. Can J Biochem. 1974;52(7):620–30. https://0-doi-org.brum.beds.ac.uk/10.1139/o74-089.

    Article  CAS  PubMed  Google Scholar 

  3. Wenzel BJ, Stults HB, Mayer J. Hypoferraemia in obese adolescents. Lancet. 1962;2(7251):327–8. https://0-doi-org.brum.beds.ac.uk/10.1016/s0140-6736(62)90110-1.

    Article  CAS  PubMed  Google Scholar 

  4. Seltzer CC, Mayer J. Serum iron and iron-binding capacity in adolescents. II. Comparison of Obese and Nonobese Subjects. Am J Clin Nutr. 1963;13:354–61. https://0-doi-org.brum.beds.ac.uk/10.1093/ajcn/13.6.354.

    Article  CAS  PubMed  Google Scholar 

  5. Nead KG, Halterman JS, Kaczorowski JM, Auinger P, Weitzman M. Overweight children and adolescents: a risk group for iron deficiency. Pediatrics. 2004;114(1):104–8. https://0-doi-org.brum.beds.ac.uk/10.1542/peds.114.1.104.

    Article  PubMed  Google Scholar 

  6. Moayeri H, Bidad K, Zadhoush S, Gholami N, Anari S. Increasing prevalence of iron deficiency in overweight and obese children and adolescents (Tehran Adolescent Obesity Study). Eur J Pediatr. 2006;165(11):813–4. https://0-doi-org.brum.beds.ac.uk/10.1007/s00431-006-0178-0.

    Article  PubMed  Google Scholar 

  7. Zhao L, Zhang X, Shen Y, Fang X, Wang Y, Wang F. Obesity and iron deficiency: a quantitative meta-analysis. Obes Rev. 2015;16(12):1081–93. https://0-doi-org.brum.beds.ac.uk/10.1111/obr.12323.

    Article  CAS  PubMed  Google Scholar 

  8. Zimmermann MB, Zeder C, Muthayya S, Winichagoon P, Chaouki N, Aeberli I, et al. Adiposity in women and children from transition countries predicts decreased iron absorption, iron deficiency and a reduced response to iron fortification. Int J Obes (Lond). 2008;32(7):1098–104. https://0-doi-org.brum.beds.ac.uk/10.1038/ijo.2008.43.

    Article  CAS  PubMed  Google Scholar 

  9. Zoroddu MA, Aaseth J, Crisponi G, Medici S, Peana M, Nurchi VM. The essential metals for humans: a brief overview. J Inorg Biochem. 2019;195:120–9. https://0-doi-org.brum.beds.ac.uk/10.1016/j.jinorgbio.2019.03.013.

    Article  CAS  PubMed  Google Scholar 

  10. Anderson GJ, Frazer DM. Current understanding of iron homeostasis. Am J Clin Nutr. 2017;106(6):1559S-1566S. https://0-doi-org.brum.beds.ac.uk/10.3945/ajcn.117.155804.

    Article  PubMed  PubMed Central  Google Scholar 

  11. Yanatori I, Kishi F. DMT1 and iron transport. Free Radic Biol Med. 2019;133:55–63. https://0-doi-org.brum.beds.ac.uk/10.1016/j.freeradbiomed.2018.07.020.

    Article  CAS  PubMed  Google Scholar 

  12. Luo C, Xu W, Tang X, Liu X, Cheng Y, Wu Y, et al. Canonical Wnt signaling works downstream of iron overload to prevent ferroptosis from damaging osteoblast differentiation. Free Radic Biol Med. 2022;188:337–50. https://0-doi-org.brum.beds.ac.uk/10.1016/j.freeradbiomed.2022.06.236.

    Article  CAS  PubMed  Google Scholar 

  13. Shawki A, Anthony SR, Nose Y, Engevik MA, Niespodzany EJ, Barrientos T, et al. Intestinal DMT1 is critical for iron absorption in the mouse but is not required for the absorption of copper or manganese. Am J Physiol Gastrointest Liver Physiol. 2015;309(8):G635–47. https://0-doi-org.brum.beds.ac.uk/10.1152/ajpgi.00160.2015.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  14. Mackenzie B, Garrick MD. Iron Imports. II. Iron uptake at the apical membrane in the intestine. Am J Physiol Gastrointest Liver Physiol. 2005;289(6):G981–6. https://0-doi-org.brum.beds.ac.uk/10.1152/ajpgi.00363.2005.

    Article  CAS  PubMed  Google Scholar 

  15. Conrad ME, Umbreit JN. Iron absorption and transport-an update. Am J Hematol. 2000;64(4):287–98. https://0-doi-org.brum.beds.ac.uk/10.1002/1096-8652(200008)64:4%3c287::aid-ajh9%3e3.0.co;2-l.

    Article  CAS  PubMed  Google Scholar 

  16. Smith KB, Smith MS. Obesity Statistics. Prim Care. 2016;43(1):121–ix. https://0-doi-org.brum.beds.ac.uk/10.1016/j.pop.2015.10.001.

    Article  PubMed  Google Scholar 

  17. Ganz T. Anemia of Inflammation. N Engl J Med. 2019;381(12):1148–57. https://0-doi-org.brum.beds.ac.uk/10.1056/NEJMra1804281.

    Article  CAS  PubMed  Google Scholar 

  18. Ng SF, Lin RC, Laybutt DR, Barres R, Owens JA, Morris MJ. Chronic high-fat diet in fathers programs β-cell dysfunction in female rat offspring. Nature. 2010;467(7318):963–6. https://0-doi-org.brum.beds.ac.uk/10.1038/nature09491.

    Article  CAS  PubMed  Google Scholar 

  19. Coimbra S, Catarino C, Santos-Silva A. The role of adipocytes in the modulation of iron metabolism in obesity. Obes Rev. 2013;14(10):771–9. https://0-doi-org.brum.beds.ac.uk/10.1111/obr.12057.

    Article  CAS  PubMed  Google Scholar 

  20. Aeberli I, Hurrell RF, Zimmermann MB. Overweight children have higher circulating hepcidin concentrations and lower iron status but have dietary iron intakes and bioavailability comparable with normal weight children. Int J Obes (Lond). 2009;33(10):1111–7. https://0-doi-org.brum.beds.ac.uk/10.1038/ijo.2009.146.

    Article  CAS  PubMed  Google Scholar 

  21. del Giudice EM, Santoro N, Amato A, Brienza C, Calabrò P, Wiegerinck ET, et al. Hepcidin in obese children as a potential mediator of the association between obesity and iron deficiency. J Clin Endocrinol Metab. 2009;94(12):5102–7. https://0-doi-org.brum.beds.ac.uk/10.1210/jc.2009-1361.

    Article  CAS  PubMed  Google Scholar 

  22. Ganz T, Nemeth E. Iron sequestration and anemia of inflammation. Semin Hematol. 2009;46(4):387–93. https://0-doi-org.brum.beds.ac.uk/10.1053/j.seminhematol.2009.06.001.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  23. Nairz M, Haschka D, Demetz E, Weiss G. Iron at the interface of immunity and infection. Front Pharmacol. 2014;5:152. https://0-doi-org.brum.beds.ac.uk/10.3389/fphar.2014.00152.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  24. Tvrda E, Peer R, Sikka SC, Agarwal A. Iron and copper in male reproduction: a double-edged sword. J Assist Reprod Genet. 2015;32(1):3–16. https://0-doi-org.brum.beds.ac.uk/10.1007/s10815-014-0344-7.

    Article  PubMed  Google Scholar 

  25. Mehta S, Goyal L, Meena ML, Gulati S, Sharma N, Harshvardhan L, et al. Assessment of pituitary gonadal axis and sperm parameters in anemic eugonadal males before and after correction of iron deficiency anemia. J Assoc Physicians India. 2018;66(9):11–2.

    PubMed  Google Scholar 

  26. Agbaraji VO, Scott RB, Leto S, Kingslow LW. Fertility studies in sickle cell disease: semen analysis in adult male patients. Int J Fertil. 1988;33(5):347–52.

    CAS  PubMed  Google Scholar 

  27. López P, Castro A, Flórez M, Miranda K, Aranda P, Sánchez-González C, et al. miR-155 and miR-122 expression of spermatozoa in obese subjects. Front Genet. 2018;9:175. https://0-doi-org.brum.beds.ac.uk/10.3389/fgene.2018.00175.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  28. Aydemir B, Kiziler AR, Onaran I, Alici B, Ozkara H, Akyolcu MC. Impact of Cu and Fe concentrations on oxidative damage in male infertility. Biol Trace Elem Res. 2006;112(3):193–203. https://0-doi-org.brum.beds.ac.uk/10.1385/BTER:112:3:193.

    Article  CAS  PubMed  Google Scholar 

  29. Grandjean V, Fourré S, De Abreu DA, Derieppe MA, Remy JJ, Rassoulzadegan M. RNA-mediated paternal heredity of diet-induced obesity and metabolic disorders. Sci Rep. 2015;5:18193. https://0-doi-org.brum.beds.ac.uk/10.1038/srep18193.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  30. Qureshi IA, Mehler MF. Emerging roles of non-coding RNAs in brain evolution, development, plasticity and disease. Nat Rev Neurosci. 2012;13(8):528–41. https://0-doi-org.brum.beds.ac.uk/10.1038/nrn3234.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  31. Gapp K, Jawaid A, Sarkies P, Bohacek J, Pelczar P, Prados J, et al. Implication of sperm RNAs in transgenerational inheritance of the effects of early trauma in mice. Nat Neurosci. 2014;17(5):667–9. https://0-doi-org.brum.beds.ac.uk/10.1038/nn.3695.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  32. Han TS, Voon DC, Oshima H, Nakayama M, Echizen K, Sakai E, et al. Interleukin 1 up-regulates MicroRNA 135b to promote inflammation-associated gastric carcinogenesis in mice. Gastroenterology. 2019;156(4):1140-1155.e4. https://0-doi-org.brum.beds.ac.uk/10.1053/j.gastro.2018.11.059.

    Article  CAS  PubMed  Google Scholar 

  33. Pinhas-Hamiel O, Newfield RS, Koren I, Agmon A, Lilos P, Phillip M. Greater prevalence of iron deficiency in overweight and obese children and adolescents. Int J Obes Relat Metab Disord. 2003;27(3):416–8. https://0-doi-org.brum.beds.ac.uk/10.1038/sj.ijo.0802224.

    Article  CAS  PubMed  Google Scholar 

  34. Yanoff LB, Menzie CM, Denkinger B, Sebring NG, McHugh T, Remaley AT, et al. Inflammation and iron deficiency in the hypoferremia of obesity. Int J Obes (Lond). 2007;31(9):1412–9. https://0-doi-org.brum.beds.ac.uk/10.1038/sj.ijo.0803625.

    Article  CAS  PubMed  Google Scholar 

  35. Gesquiere I, Foulon V, Augustijns P, Gils A, Lannoo M, Van der Schueren B, et al. Micronutrient intake, from diet and supplements, and association with status markers in pre- and post-RYGB patients. Clin Nutr. 2017;36(4):1175–81. https://0-doi-org.brum.beds.ac.uk/10.1016/j.clnu.2016.08.009.

    Article  CAS  PubMed  Google Scholar 

  36. Brasse-Lagnel C, Karim Z, Letteron P, Bekri S, Bado A, Beaumont C. Intestinal DMT1 cotransporter is down-regulated by hepcidin via proteasome internalization and degradation. Gastroenterology. 2011;140(4):1261-1271.e1. https://0-doi-org.brum.beds.ac.uk/10.1053/j.gastro.2010.12.037.

    Article  CAS  PubMed  Google Scholar 

  37. Mena NP, Esparza A, Tapia V, Valdés P, Núñez MT. Hepcidin inhibits apical iron uptake in intestinal cells. Am J Physiol Gastrointest Liver Physiol. 2008;294(1):G192–8. https://0-doi-org.brum.beds.ac.uk/10.1152/ajpgi.00122.2007.

    Article  CAS  PubMed  Google Scholar 

  38. Woloshun RR, Yu Y, Xu X, Lee JK, Zhu S, Shine JS, et al. Four AAs increase DMT1 abundance in duodenal brush-border membrane vesicles and enhance iron absorption in iron-deprived mice. Blood Adv. 2022;6(10):3011–21. https://0-doi-org.brum.beds.ac.uk/10.1182/bloodadvances.2021005111.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  39. Yuxin L, Chen L, Xiaoxia L, Yue L, Junjie L, Youzhu L, et al. Research progress on the relationship between obesity-inflammation-aromatase axis and male infertility. Oxid Med Cell Longev. 2021;2021:6612796. https://0-doi-org.brum.beds.ac.uk/10.1155/2021/6612796.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  40. Akhter MS, Hamali HA, Iqbal J, Mobarki AA, Rashid H, Dobie G, et al. Iron deficiency anemia as a factor in male infertility: awareness in health college students in the Jazan Region of Saudi Arabia. Int J Environ Res Public Health. 2021;18(24):12866. https://0-doi-org.brum.beds.ac.uk/10.3390/ijerph182412866.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  41. Barbagallo F, Condorelli RA, Mongioì LM, Cannarella R, Cimino L, Magagnini MC, et al. Molecular mechanisms underlying the relationship between obesity and male infertility. Metabolites. 2021;11(12):840. https://0-doi-org.brum.beds.ac.uk/10.3390/metabo11120840.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  42. Wagner IV, Klöting N, Atanassova N, Savchuk I, Spröte C, Kiess W, et al. Prepubertal onset of obesity negatively impacts on testicular steroidogenesis in rats. Mol Cell Endocrinol. 2016;437:154–62. https://0-doi-org.brum.beds.ac.uk/10.1016/j.mce.2016.08.027.

    Article  CAS  PubMed  Google Scholar 

  43. Zhao JL, Zhao YY, Zhu WJ. A high-fat, high-protein diet attenuates the negative impact of casein-induced chronic inflammation on testicular steroidogenesis and sperm parameters in adult mice. Gen Comp Endocrinol. 2017;252:48–59. https://0-doi-org.brum.beds.ac.uk/10.1016/j.ygcen.2017.07.013.

    Article  CAS  PubMed  Google Scholar 

  44. Zhang FL, Yuan S, Dong PY, Ma HH, De Felici M, Shen W, et al. Multi-omics analysis reveals that iron deficiency impairs spermatogenesis by gut-hormone synthesis axis. Ecotoxicol Environ Saf. 2022;248: 114344. https://0-doi-org.brum.beds.ac.uk/10.1016/j.ecoenv.2022.114344.

    Article  CAS  PubMed  Google Scholar 

  45. Tsao CW, Liao YR, Chang TC, Liew YF, Liu CY. Effects of iron supplementation on testicular function and spermatogenesis of iron-deficient rats. Nutrients. 2022;14(10):2063. https://0-doi-org.brum.beds.ac.uk/10.3390/nu14102063.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  46. Fullston T, Ohlsson-Teague EM, Print CG, Sandeman LY, Lane M. Sperm microRNA content is altered in a mouse model of male obesity, but the same suite of microRNAs are not altered in offspring’s sperm. PLoS ONE. 2016;11(11): e0166076. https://0-doi-org.brum.beds.ac.uk/10.1371/journal.pone.0166076.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  47. Yuan S, Liu Y, Peng H, Tang C, Hennig GW, Wang Z, et al. Motile cilia of the male reproductive system require miR-34/miR-449 for development and function to generate luminal turbulence. Proc Natl Acad Sci U S A. 2019;116(9):3584–93. https://0-doi-org.brum.beds.ac.uk/10.1073/pnas.1817018116.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  48. Kuang W, Zhang J, Lan Z, Deepak RNVK, Liu C, Ma Z, et al. SLC22A14 is a mitochondrial riboflavin transporter required for sperm oxidative phosphorylation and male fertility. Cell Rep. 2021;35(3): 109025. https://0-doi-org.brum.beds.ac.uk/10.1016/j.celrep.2021.109025.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  49. Ward GE, Vacquier VD. Dephosphorylation of a major sperm membrane protein is induced by egg jelly during sea urchin fertilization. Proc Natl Acad Sci U S A. 1983;80(18):5578–82. https://0-doi-org.brum.beds.ac.uk/10.1073/pnas.80.18.5578.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  50. O’Flaherty C, de Lamirande E, Gagnon C. Positive role of reactive oxygen species in mammalian sperm capacitation: triggering and modulation of phosphorylation events. Free Radic Biol Med. 2006;41(4):528–40. https://0-doi-org.brum.beds.ac.uk/10.1016/j.freeradbiomed.2006.04.027.

    Article  CAS  PubMed  Google Scholar 

  51. Scheffler K, Uraji J, Jentoft I, Cavazza T, Mönnich E, Mogessie B, et al. Two mechanisms drive pronuclear migration in mouse zygotes. Nat Commun. 2021;12(1):841. https://0-doi-org.brum.beds.ac.uk/10.1038/s41467-021-21020-x.

    Article  CAS  PubMed  PubMed Central  Google Scholar 

  52. Yang J, Wu G, Feng Y, Lv Q, Lin S, Hu J. Effects of taurine on male reproduction in rats of different ages. J Biomed Sci. 2010;171 Suppl 1(Suppl 1):S9. https://0-doi-org.brum.beds.ac.uk/10.1186/1423-0127-17-S1-S9.

    Article  CAS  Google Scholar 

  53. Laurinyecz B, Péter M, Vedelek V, Kovács AL, Juhász G, Maróy P, et al. Reduced expression of CDP-DAG synthase changes lipid composition and leads to male sterility in Drosophila. Open Biol. 2016;6(1):50169. https://0-doi-org.brum.beds.ac.uk/10.1098/rsob.150169.

    Article  CAS  PubMed  Google Scholar 

  54. Francou MM, Hombrebueno JR, De Juan J. Identification and cellular location of glutamine synthetase in human sperm. Cell Tissue Res. 2012;350(1):183–7. https://0-doi-org.brum.beds.ac.uk/10.1007/s00441-012-1465-x.

    Article  CAS  PubMed  Google Scholar 

  55. Tas GG, Soygur B, Kutlu O, Sati L. A comprehensive investigation of human endogenous retroviral syncytin proteins and their receptors in men with normozoospermia and impaired semen quality. J Assist Reprod Genet. 2023;40(1):97–111. https://0-doi-org.brum.beds.ac.uk/10.1007/s10815-022-02673-z.

    Article  PubMed  Google Scholar 

  56. Srivastava S, Desai P, Coutinho E, Govil G. Mechanism of action of L-arginine on the vitality of spermatozoa is primarily through increased biosynthesis of nitric oxide. Biol Reprod. 2006;74(5):954–8. https://0-doi-org.brum.beds.ac.uk/10.1095/biolreprod.105.046896.

    Article  CAS  PubMed  Google Scholar 

Download references

Acknowledgements

We would like to thank Chenjing Duan (Xi’an Jiaotong University Health Science Centre) for providing advice regarding our work.

Funding

This work was supported as part of the Innovation Capability Support Program of Shaanxi (No. 2021PT-050) with the funder Ying Xue, and the Foundation of the First Affiliated Hospital of Xi’an Medical University (XYFYPT-2023–03) with the funder Yun Ye.

Author information

Authors and Affiliations

  1. Laboratory Animal Center, Xi’an Jiaotong University Health Science Centre, Xi’an, 710061, China

    Yanru Zhang, Ruike Ding, Yulin Zhang, Jia Qi, Wenbin Cao, Lin Zhou, Ying Xue & Enqi Liu

  2. Spring Biological Technology Development Co., Ltd, Fangchenggang, Guangxi, 538000, China

    Lijun Deng

  3. Central Laboratory, The First Affiliated Hospital of Xi’an Medical University, Xi’an, 710000, China

    Yun Ye

  4. Key Laboratory of Environment and Genes Related to Diseases, Ministry of Education of China, Xi’an, 710049, China

    Enqi Liu

Authors
  1. Yanru Zhang
    View author publications

    You can also search for this author in PubMed Google Scholar

  2. Ruike Ding
    View author publications

    You can also search for this author in PubMed Google Scholar

  3. Yulin Zhang
    View author publications

    You can also search for this author in PubMed Google Scholar

  4. Jia Qi
    View author publications

    You can also search for this author in PubMed Google Scholar

  5. Wenbin Cao
    View author publications

    You can also search for this author in PubMed Google Scholar

  6. Lijun Deng
    View author publications

    You can also search for this author in PubMed Google Scholar

  7. Lin Zhou
    View author publications

    You can also search for this author in PubMed Google Scholar

  8. Yun Ye
    View author publications

    You can also search for this author in PubMed Google Scholar

  9. Ying Xue
    View author publications

    You can also search for this author in PubMed Google Scholar

  10. Enqi Liu
    View author publications

    You can also search for this author in PubMed Google Scholar

Contributions

Ying Xue and Enqi Liu conceived and designed this study. Yanru Zhang was responsible for the first draft of the manuscript and the figures. Yanru Zhang and Ringke Ding were in charge of data analysis, Yuling Zhang and Jia Qi were in charge of animal handling. Material preparation and data collection were performed by Wenbin Cao and Ruike Ding; Lijun Deng and Lin Zhou were responsible for software and visualization. Ying Xue, Enqi Liu, Yanru Zhang, and Yun Ye reviewed the manuscript. All authors have read and agreed to the published version of the manuscript.

Corresponding authors

Correspondence to Ying Xue or Enqi Liu.

Ethics declarations

Ethics approval and consent to participate

The study was approved by the Animal Experimental Ethics Committee of Xi’an Jiaotong University.

Consent for publication

Not applicable.

Competing interests

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/.

Reprints and permissions

About this article

Check for updates. Verify currency and authenticity via CrossMark

Cite this article

Zhang, Y., Ding, R., Zhang, Y. et al. Dysfunction of DMT1 and miR-135b in the gut-testis axis in high-fat diet male mice. Genes Nutr 19, 1 (2024). https://0-doi-org.brum.beds.ac.uk/10.1186/s12263-024-00737-6

Download citation

  • Received:

  • Accepted:

  • Published:

  • DOI: https://0-doi-org.brum.beds.ac.uk/10.1186/s12263-024-00737-6

Keywords

Genes & Nutrition

ISSN: 1865-3499

Contact us