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Review

Maternal Mineral Nutrition Regulates Fetal Genomic Programming in Cattle: A Review

by
Muhammad Anas
1,*,
Wellison J. S. Diniz
2,*,
Ana Clara B. Menezes
3,
Lawrence P. Reynolds
1,
Joel S. Caton
1,
Carl R. Dahlen
1 and
Alison K. Ward
4
1
Department of Animal Sciences, Center for Nutrition and Pregnancy, North Dakota State University, Fargo, ND 36849, USA
2
Department of Animal Sciences, Auburn University, Auburn, AL 36849, USA
3
Department of Animal Science, South Dakota State University, Brookings, SD 57007, USA
4
Department of Veterinary Biomedical Sciences, University of Saskatchewan, Saskatoon, SK S7N 5B4, Canada
*
Authors to whom correspondence should be addressed.
Metabolites 2023, 13(5), 593; https://doi.org/10.3390/metabo13050593
Submission received: 4 April 2023 / Revised: 22 April 2023 / Accepted: 24 April 2023 / Published: 26 April 2023
(This article belongs to the Special Issue Mineral and Energy Metabolism of Mammals during Pregnancy)
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Abstract

:
Maternal mineral nutrition during the critical phases of fetal development may leave lifetime impacts on the productivity of an individual. Most research within the developmental origins of the health and disease (DOHaD) field is focused on the role of macronutrients in the genome function and programming of the developing fetus. On the other hand, there is a paucity of knowledge about the role of micronutrients and, specifically, minerals in regulating the epigenome of livestock species, especially cattle. Therefore, this review will address the effects of the maternal dietary mineral supply on the fetal developmental programming from the embryonic to the postnatal phases in cattle. To this end, we will draw a parallel between findings from our cattle model research with data from model animals, cell lines, and other livestock species. The coordinated role and function of different mineral elements in feto-maternal genomic regulation underlies the establishment of pregnancy and organogenesis and, ultimately, affects the development and functioning of metabolically important tissues, such as the fetal liver, skeletal muscle, and, importantly, the placenta. Through this review, we will delineate the key regulatory pathways involved in fetal programming based on the dietary maternal mineral supply and its crosstalk with epigenomic regulation in cattle.

1. Introduction

The mechanisms and the interaction of processes in the growth of an individual from embryonic to adult life is investigated in the field of developmental biology [1,2]. Rigorous research over the last half of a century has led to an emergence of reports that conjoin developmental biology with the areas of genetics [3], evolution [4], and epidemiology [5,6,7]. This impact on developmental biology, specifically in the area of epidemiology, has resulted in the formulation of a concept and, ultimately, a separate discipline, namely, fetal programing or the developmental origins of health and disease (DOHaD), first articulated by the human epidemiologist Dr. David Barker and colleagues [8].
The concept of the DOHaD hypothesis was not new at that time and can be traced back to the idea from the early 1800s of organic evolution, the concept that the adopted physical changes in one generation are transferable to subsequent generations via gametes, by Lamarck [9]; however, Barker was among the first to coin the term “fetal programming” or “developmental origins of health and disease”. Widdowson and McCance [10] were among the first cell biologists who provided evidence that there are some critical phases in development, especially during the pre-weaning period, in which undernutrition leads to changes in growth and development in rats. However, later evidence by Barker [8] and others in this emerging discipline suggested that fetal growth during pregnancy is regulated by numerous factors that, in turn, regulate genetic and epigenetic pathways [11,12]. Maternal nutrient intake during gestation is one of the major factors. The nutrients available to the conceptus not only affect the expression of the fetal and placental genomes but also significantly impact offspring growth postnatally [12,13].
Apart from human and laboratory animal model research [14,15], different studies have linked the concept of developmental programming to livestock performance, including cattle [16,17,18,19], sheep [20,21], and pigs [22,23]. Furthermore, some literature reviews [24,25,26,27,28] have pointed out the role of micronutrients in epigenome regulation, which leads to developmental programming. These ideas are the basis of developmental plasticity, defined as fetal adaptations to an altered intrauterine environment at the expense of postnatal developmental prospects [29]. Nutritional manipulations during times of developmental plasticity, i.e., embryonic, fetal, or neonatal life, exert either short or long-term effects on the development of muscle, adipose tissue, and ovarian reserves and the overall longevity of the offspring [13,30,31,32,33,34]. Based on these studies and some recent livestock modeling [35,36], it seems that nutritional alterations do affect metabolic disorders in humans or model organisms and may have equal or more severe impacts on cow–calf, feedlot, and dairy production systems in the livestock sector.
The influence of macronutrients such as carbohydrates, proteins, and lipids has been researched and reviewed several times [17,25,37,38,39], with data extending to the omics level to investigate their regulatory roles in epigenomics and metabolomics [18,19,20,33,40]. In contrast, very little is known about their effects on the maternal dietary mineral supply and their regulatory role(s) in programming genomic function and fetal development. Although minerals are required in a smaller amount than macronutrients, their deficiency can lead to a significant reduction in growth and development [41]. Moreover, an excess of minerals can lead to toxicity. The mineral requirements of beef and dairy cattle along with the maximum tolerable limits are shown in Table 1 [42,43,44]. In this review, our objective is to summarize the key role of essential macro- and microminerals in fetal epigenome programming.

2. Fetal Programming as a Multifactorial System

Although much of the research in fetal programming has focused on insults during mid- and late gestation, there is a growing interest in the earlier stages of gestation, which may “set the stage” for later programming events. Although most of the fetal size increase takes place in the last trimester, the first third of gestation is a critical period for organogenesis and tissue hyperplasia, as well as placentation [21,34,45,46], as shown in Figure 1. The prenatal growth trajectory of the conceptus is controlled by maternal nutrition either directly, by the provision of the essential nutrients; indirectly, via placental function, which regulates the transport of these nutrients [47]; or by altering the epigenetic mechanisms [48,49,50,51].
Pregnancy recognition occurs 15 to 16 days after estrous in cattle [58] and initiates maternal uterine vasculature changes to allow for the proper respiratory gas exchange and nutrient transfer to the developing embryo. Pregnancy is associated with a significant decrease in CpG methylation at the Sp1 promotor region of the KCNMB1 gene (potassium calcium-activated channel subfamily M regulatory Beta subunit 1) and an increase in the expression of large-conductance Ca+2-activated K+ channel receptors, BKCa, causing uterine artery dilation [59]. The expression of KCNMB1 is also regulated by an increase in the expression of estrogenic receptor alpha [60] and the maintenance of membrane potential by K+ and Ca+2 ions to cause pregnancy-associated relaxation by reducing the myogenic tone [61,62] (Figure 2). In addition, estrogen is a potent angiogenic factor in the uterus and is involved in systemic cardiovascular changes during pregnancy (e.g., increased cardiac output [63,64]).
The development of fetal organs is significantly affected by mineral availability [65]. Zinc deficiency or excess during pregnancy can impact the development of multiple organs, including the brain, lungs, skeleton, and heart [66,67,68,69]. In the case of brain development, zinc deficiency impairs the function of Zic (Zinc finger proteins of the cerebellum) genes [70], which are essential for cerebellar development [70,71,72]. Zinc supranutrition (the supplementation of more than the normal requirement but less than the maximum tolerable limit) has shown the potential to enhance the cognitive ability of offspring in rats by increasing the expression of the signal transducer and activator of transcription 3 (STAT3) and matrix metalloproteinase-2/9 (MMP-2/9) [69]. STAT3-MMP-2/9 activity promotes the invasion and migration of placental trophoblast cells and improves neural function [69,73]. In heart development, zinc deficiency alters the distribution of human natural killer-1 (HNK-1) cells and connexin 43 (Cx43) in the myocardium, contributing to the development of cardiovascular anomalies [74,75].
Like zinc, copper deficiency and supranutrition are associated with oxidative distress and neural degenerative disorders [76,77]. It has also been observed that both copper deficiency and the improper absorption of copper from the rumen in cattle can lead to such conditions. This can be due to the accessibility of molybdenum and sulfur, resulting in the formation of thiomolybdates, which can bind with copper in the rumen leading to inappropriate copper availability [78]. Copper deficiency leads to the suppression of the activity of a cuproenzyme, cytochrome-c oxidase, in the red nucleus region associated with large motor neurons, causing enzootic ataxia or swayback in lambs [79,80]. In addition, supranutritional levels of of copper, along with zinc, cobalt, and manganese, enhance the expression of metallothionein 1A (MT1A) in the dam and Cu-Zn superoxide dismutase (CU/Zn SOD) in developing offspring of cattle [77]. The MT1A is the major transporter of metal ions and CU/Zn SOD is involved in the regulation of oxidative stress and neurodegenerative disorder [77,81].
Selenium has biological functions via selenoproteins [28,82]. A maternal Se supplementation has effects on reproduction and developmental outcomes, which may be mediated by epigenetic events [28,83]. Selenium deficiency decreases the expression of selenoproteins, such as glutathione peroxidases, including GPx1, GPx2, GPx4, and SELENOP, including Selenoprotein-P, leading to alterations in embryonic development, oxidative stress mechanisms, reproductive development, and male fertility, respectively [84,85]. Maternal Se deficiency is associated with pancreatic atrophy in the developing fetus [86]. Moreover, maternal Se deficiency causes an elevation in the selenoenzyme type II deiodinase (Dio2), which reduces thyroxine production (Figure 3). On the other hand, supranutritional Se enhances thyroxine levels and impairs the growth hormone, insulin-like growth factor (GH-IGF) system [87,88]. The GH-IGF system impairment causes glucose intolerance and hypo-insulinemia in the fetus [86].
In cattle, primary and secondary myogenesis during the early fetal period start at days 47 and 119, respectively, and establish the lifetime potential for muscle development (see Figure 1) [56,93,94]. This is why there is no net increase in the number of muscle fibers after birth. Myogenesis requires the binding of active thyroid hormones to its receptors [95,96], especially thyroid receptor α, which is predominantly expressed in skeletal muscle [97] and is involved in promoting angiogenesis [98,99]. The deficiency of selenium, zinc, and iron can cause the impairment of thyroid hormone synthesis and action [100] by decreasing the expression of glutathione peroxidase (a selenoprotein) [101], 1,5′-deiodinase [102], and thyroperoxidase [103], respectively. Iron deficiency causes iron deficiency anemia, which reduces the activity of thyroid peroxidase (a Fe-dependent enzyme), leading to the repression of thyroid hormone synthesis and myogenesis [104].
Fetal skeletal development and bone mineralization are affected by maternal mineral status. Severe hypocalcemia, hypophosphatemia [105,106], and hypomagnesemia [107,108] are associated with reduced levels of parathyroid hormone (PTH) (Figure 4). Normally, PTH acts on PTH receptor 1 (PTHR1) of the kidney, which activates cyclic adenosine monophosphate (cAMP)-associated pathways and requires Mg+2 as a cofactor [109,110] for calcitriol (1,25(OH)D) and vitamin D production. However, a decrease in PTH leads to vitamin D deficiency [111], which ultimately affects bone formation and mineralization in the developing fetus [107]. Both hypo- and hypercalcemic dams were associated with the upregulation of fatty acid binding protein 4 (FABP4), fatty acid synthase (FASN), and acetyl coenzyme A carboxylase 1 (ACC1) in the adipose tissue and liver of the offspring, leading to dyslipidemia and bone demineralization to maintain the serum level of calcium in the offspring [112].

3. The Roles of Minerals in Fetal Genome Regulation

Epigenomic regulation in the fetus is affected by the insufficiency of maternal nutrients, including minerals. In a recent study in cattle, the authors reported that essential micronutrient supplementation and the dietary plane of nutrition (as assessed by the rate of bodyweight gain) during early gestation can affect the neonatal immune response and the availability of mineral reserves for postnatal development [114,115]. In addition, the expression of genes associated with cholesterol synthesis, ion homeostasis, and nutrient transport was altered in the developing placenta [116,117]. To explain the epigenomic regulation of these pathways based on maternal mineral homeostasis and their effects on fetal programming, different studies have been conducted in model organisms (see Table 2).
The transcriptomics of the developing fetus can be regulated either by changing the methylation pattern of specific DNA regions or by repressing mRNA expression based on the adequacy of maternal mineral nutrition. For example, Zn is transported in the blood by forming a complex with metallothionein-2 (MT2) [126]. In a mouse model, Zn deficiency was associated with a polymorphism in MT2 at rs1610216 (MT2A–209A/G) along with histone modification and hypermethylation of a metal-responsive element (MRE) in the promotor region of MT2 [123], and similar changes are seen in human [127]. Furthermore, the mRNA expression of zinc transporter 1 (ZnT1) in a zebrafish model [128], as well as zinc importing protein (ZIP14) in a rat model [75], and divalent metal transporter 1 (DMT1) in human cell lines [129] is associated with the availability of zinc. The impairment of the expression of these genes affects zinc availability to the developing fetus and, subsequently, organogenesis [66,67].
Selenium deficiency affects the expression of selenoenzymes such as GPx1, GPx2, and GPx4 and selenoproteins (i.e., Selenoproteins-P, SELENOP), which are involved in not only fetal reproductive development and the regulation of oxidative stress [84,85] but also the overall DNA methylation pattern. Selenium availability affects the concentration of S-adenosyl homocysteine (a potential inhibitor of DNA methyltransferases) and the availability of S-adenosyl methionine (the methyl-donor for all methylation reactions) in the methionine–homocysteine cycle [130,131,132,133]. In a rainbow trout model, selenium availability affected the differentially methylated cytosines of more than 6500 differentially methylated genes associated with immune modulations and neural signaling [124].
Like zinc and selenium deficiency, maternal iron deficiency in pregnancy is critical as it can permanently affect brain development [120,121]. Iron deficiency is associated with histone modification and DNA methylation at the brain-derived neurotrophic factor IV (BDNF-IV) promotor region in the hippocampus of the developing fetus, which affects cognitive response and hippocampal plasticity, as observed in a rat model [120]. Additionally, iron deficiency causes a reduction in the expression of DMT1 (a major transporter) in rats, which leads to impaired manganese availability to the developing fetus [134,135]. Copper deficiency can also impair DMT1 expression and affect the availability of iron and manganese to the fetus [136] (Figure 5). In a study of copper availability and DNA methylation changes in fetuses during pregnancy in humans, the most robust negatively associated, differentially methylated region was found in a zinc-finger gene, ZNF197, which was correlated with birth weight [125].
In terms of macrominerals, maternal magnesium deficiency and calcium deficiency affect the methylation of CpG island regions of hydroxysteroid 11-beta dehydrogenase 2 (Hsd11b2) [119] and hydroxysteroid 11-beta dehydrogenase 1 (Hsd11b1) [118], respectively, leading to the impairment of glucocorticoid metabolism in the developing fetus. The hepatic glucocorticoid concentration was altered in rats [119], which affects the GH-IGF system, leading to a reduction in postnatal skeletal development and myogenesis [95,96]. Due to sex-specific modifications, however, the effects of insulin resistance were minimal in later F2 and F3 generations, although insulin production was still dysregulated [140,141].

4. Feto-Maternal Crosstalk

After attachment/implantation, fetomaternal crosstalk and the transport of nutrients (including minerals) are completely dependent on the placenta. Before placental vascularization is completed (the first 50 d of gestation in cattle), histotrophic nutrition (via uterine secretions) is the main source of nutrients to the fetus [21]. However, after placental circulation is established, hemotrophic nutrition is the primary pathway involved in the transfer of nutrients to the fetus. In ruminants, chorionic development begins at about day 20 of pregnancy, and placental development along with the interdigitation of fetomaternal villi completes at day 50 [46]. The establishment of pregnancy requires minerals and is especially associated with membrane potential as regulated by estrogen, K+, and Ca+2 [61,62]. In ewes, Ca+2 and Na+ levels increase in histotroph on post-fertilization from days 13 to 16, suggesting their role in placental development and implantation [142]. During pregnancy, estrogen binds to the SP1 site in the promotor of the KCNMB1 gene, which causes upregulation in the expression of BKCa [61]. The opening of BKCa channels results in the efflux of K+ and the sarcoplasmic release of Ca+2 to further enhance KCNMB1 expression and BKCa channels [59], which causes the pregnancy-induced relaxation of uterine vascular smooth muscle. This hypothesis was further strengthened in cattle models by one recent study in which sarcoplasmic reticulum Ca+2-ATPase 3 (ATP2A3) and ATPase subunit beta-1 (ATP1B1) were found to be upregulated in caruncles of the mineral-supplemented group compared to the non-supplemented one, indicating the intracellular sarcoplasmic Ca+2 release through these ATPase pumps [116].
The placental transport of other micro- and macrominerals is required for fetal developmental programming. Zinc is maternally transported by ZnT1 in the form of the Zn-MT complex [126] and binds to ZIP14 in placental trophoblast. It is further transported to the fetus by ZnT2 and DMT1 [126] (Figure 5). When zinc and copper supplementation and cobalt and manganese in beef cattle were examined together, MT1A expression was found upregulated in the dams and Cu/Zn SOD levels were upregulated in their successive offerings [77]. This explains the maternal pathway for zinc transport, but the transport mechanism of zinc in the fetus still needs validation in the cattle model. The cattle model study, however, recently showed evidence supporting fetal transport. It was found that the metallothionein coding genes MT1A, MT2A, and MT1E are upregulated, while ZnT10 is differentially expressed in mineral-supplemented fetal groups compared to non-supplemented groups [117].
Selenium and iodine deficiency can impair fetal development by influencing the GH-IGF system [87,91]. In the maternal liver, selenium in the presence of selenophosphate synthetase and SEPSECS (Sep [O-Phosphoserine]) TRNA:Sec ([Selenocysteine TRNA Synthase]) is converted into selenophosphate and selenocyctenyl tRNA, respectively. Selenocyctenyl tRNA in the presence of SBP (selenocysteine binding protein 2) produces selenoproteins, such as SELENOP, and deiodinases [89]. SELENOP binds to ApoER2 (Apolipoprotein E Receptor-2) in the placental trophoblast and is transported to the fetus [85,90]. The production of Dio2 converts the Thyroxine-4 (T4) to active triiodothyronine (T3) [89]. T3 and T4 are produced in the fetal thyroid gland by thyroglobulin produced from iodine and tyrosine [91]. Free T3 increases the expression of Dio3 in placental trophoblast, which will convert T3 back to inactive T4 in the fetus. This mechanism is associated with low active T3 in the fetus and, thus, prevents fetal hyperthyroidism [92] (Figure 3). The proposed mechanism of selenium feto-maternal transport based on lab animal data was not validated in a lamb model, and no changes in fetal T3:T4 were identified when ewes were supplemented with selenium [88]. This puts a question mark on the role of Dio3 in the interconversion of T3 to T4 in fetuses, indicating the current lack of understanding regarding fetal selenium transport.
Placental transporters are regulated by minerals, including manganese, iron, and copper, as shown in Figure 5. Manganese or iron in blood serum forms a complex with transferrin (Tf) proteins. This complex interacts with the transferrin 1 receptor (TfR1) at the placental microvillous membrane and is endocytosed in vesicle form [135,137]. This proposed pathway of the manganese/iron-Tf complex binding to TfR1 for vesicular endocytosis was also supported in a recent cattle model study, in which TfR1 was differentially expressed in the minerals-supplemented group compared to the non-supplemented group [117]. The acidification of these vesicles causes the release of either manganese or iron, which is further transported to the fetus by DMT1 [135,137,139,143,144]. The fetal uptake of Cu is performed by the binding of Cu+2 from maternal plasma to a high-affinity copper transporter protein 1, CTR1, at the placental trophoblast [145]. The transfer of Cu from CTR1 to a chaperon protein, ATOX1, is associated with the transport to either the fetus by the ATPase ATP7A or back to the dam and then the maternal liver by the ATPase ATP7B [138,139]. Copper supplementation data in a cattle model have shown that, rather than CTR1, MTIA and Cu/Zn SOD can be the maternal and fetal transporters of copper, respectively [77,146], emphasizing the need for further research on copper deficiency in a cattle model.
The transport and regulation of some macrominerals such as magnesium, calcium, and phosphorous are interlinked and are affected by the availability of each in the maternal diet (Figure 4). Calcium from blood plasma interacts with the calcium-sensing receptor (CaSR) at the placenta and increases the expression of placental parathyroid hormone-related proteins (PTHrP) and the release of parathyroid hormone (PTH) from the fetal parathyroid gland [105,113]. PTHrP expression increases in the maternal mammary tissues of humans; thus, both calcium-associated mechanisms run parallel in the fetal and maternal systems [111]. Both PTH and PTHrP from the fetus and PTHrP from the dam act on PTH receptor 1 (PTHR1) of the kidney both in the fetus and dam, which activates cyclic adenosine monophosphate (cAMP)-associated pathways and requires Mg+2 as a cofactor [109,110]. The cAMP-associated pathways increase the expression of 25(OH)D(3)-1-α hydroxylase, which then increases calcitriol production from 25(OH)D3, resulting in calcium and phosphorous absorption from the intestine [110,111]. Based on these mechanisms, the deficiency of any of these minerals—magnesium, calcium, or phosphorous—will affect the availability of each other and, ultimately, affect bone mineralization and development in the fetal and maternal systems.

5. Final Considerations

The potential regulatory roles of maternal mineral intake in developmental programming, from conception to birth, indicate that the excess or deficiency of minerals can lead to pre- and postnatal metabolic disorders and growth abnormalities [147]. The limitation of the studies we have cited is that most are based primarily on laboratory animal models. Although there is a need to validate these observations more extensively and in other species, basic epigenomic regulation involves similar patterns in most species, and, as such, similar responses are expected in cattle and other livestock models [148,149,150]. Recent studies using cattle as experimental models [18,19,114,115,116] have provided evidence that maternal nutrition during early pregnancy affects the deposition of minerals for postnatal development, metal ion homeostasis, growth regulatory pathways (e.g., the GH-IGF and thyroid hormone pathways), and, in particular, the overall metabolomics of the developing fetus. Based on animal models, and despite the limited evidence from livestock models [116,117], we believe that the proposed mechanisms are very likely to be valid but still need to be examined in livestock models of mineral deficiency or excess. Moreover, the literature concerning sheep [88] and cattle [77,146] models still brings into question the accepted pathways of feto-maternal transport, especially for selenium, zinc, and copper.
Another major limitation is that the available data are mostly based on mRNA, which is insufficient to make conclusions about epigenomic regulation and its role in fetal programming. In this review, we have presented some key genomic/molecular regulatory pathways involved in the effects of minerals on the epigenetic regulation of fetal and placental development. However, much more information and a much better understanding of the alterations in gene expression and their association with epigenetic signals (i.e., non-coding RNAs, histone modifications, and DNA methylation patterns) are needed in other species models. Recent reviews have done a good job explaining the role of epigenetic signals in the effects of maternal and paternal stressors on the developing embryo and fetus [34,151]. The effects of these stressors, however, across the offspring’s lifetime and across subsequent generations warrant further investigation. In addition, many of the mineral deficiencies regulate the GH-IGF and thyroid hormone systems; however, the compensatory adaptations of subsequent generations to maternal and postnatal stressors in terms of epigenetic signal inheritance need to be explored further [140].
Future studies are needed to address these abovementioned limitations in the available data to gain a better understanding of maternal mineral nutrition and its role in the epigenetic regulation of the developing fetus and offspring. Furthermore, we also need to identify efficient ways to correlate the epigenomic signaling data (i.e., the DNA methylation pattern, histone modifications, or non-coding RNAs) with genomic regulation, so that we can effectively translate the effects of maternal nutrition and other prenatal stressors across generations by delineating the cascade of minerals and mineral transporters involved in feto-maternal crosstalk. However, based on the available literature from animal models (including livestock species), humans, and cell lines, we have discussed our current understanding of the genomic regulatory roles of the following:
  • Calcium in dyslipidemia and insulin resistance;
  • Zinc in neural, cardiac, and general organ development and trace mineral transport;
  • Selenium in reproductive function, the regulation of the GH-IGF system, and the thyroid hormone system;
  • Magnesium in glucocorticoid metabolism;
  • Copper in oxidative stress, the regulation of the GH-IGF system, and placental development;
  • Calcium and potassium in the establishment of pregnancy and the regulation of placental vascular tone;
  • Selenium and iron in growth hormone metabolism and myogenesis;
  • Magnesium, calcium, and phosphorous in skeletal development and parathyroid hormone and vitamin D metabolism.

Author Contributions

M.A., A.K.W. and W.J.S.D. conceived the work. M.A. wrote the first draft. M.A., W.J.S.D., A.C.B.M., L.P.R., J.S.C., C.R.D. and A.K.W., have contributed to the to the critical reading, and editing of the manuscript. All authors have read and agreed to the published version of the manuscript.

Funding

This was funded by the North Dakota Agricultural Experiment Station (NDAES), the North Dakota State Board of Agricultural Research and Education (SBARE)–grant number 19-23-0155, and by Purina Animal Nutrition LLC, Gray Summit, MO, USA. M.A. was financially supported by the Higher Education Commission (HEC) of Pakistan, through the US-Pakistan Knowledge Corridor program. W.J.S.D. was financially supported by the Agricultural Research Service, U.S. Department of Agriculture, under Agreement No. 58-6010-1-005, by the Alabama Agricultural Experiment Station—Hatch program of the National Institute of Food and Agriculture, U.S. Department of Agriculture.

Acknowledgments

The authors would like to thank our colleagues, including undergraduate and graduate students and postdoctoral fellows for their dedication. We also thank the many laboratory and farm personnel who have made such important contributions to these efforts.

Conflicts of Interest

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

References

  1. Minelli, A. Animal Development, an Open-Ended Segment of Life. Biol. Theory 2011, 6, 4–15. [Google Scholar] [CrossRef]
  2. Love, A.C. Explaining the Ontogeny of Form: Philosophical Issue; Wiley Online Library: Hoboken, NJ, USA, 2008. [Google Scholar]
  3. Badyaev, A.V. Maternal Effects as Generators of Evolutionary Change: A Reassessment. Ann. N. Y. Acad. Sci. 2008, 1133, 151–161. [Google Scholar] [CrossRef] [PubMed]
  4. Lafuente, E.; Beldade, P. Genomics of Developmental Plasticity in Animals. Front. Genet. 2019, 10, 720. [Google Scholar] [CrossRef] [PubMed]
  5. Liu, S.; Jones, R.N.; Glymour, M.M. Implications of Lifecourse Epidemiology for Research on Determinants of Adult Disease. Public Health Rev. 2010, 32, 489–511. [Google Scholar] [CrossRef] [PubMed]
  6. Arima, Y.; Fukuoka, H. Developmental Origins of Health and Disease Theory in Cardiology. J. Cardiol. 2020, 76, 14–17. [Google Scholar] [CrossRef] [PubMed]
  7. Barker, D.J.P. Mothers, Babies and Disease in Later Life. BMJ 1994, 310, 180. [Google Scholar]
  8. Barker, D.J.P. The Fetal and Infant Origins of Adult Disease. BMJ 1990, 301, 1111. [Google Scholar] [CrossRef]
  9. Prentice, A.M.; Moore, S.E. Early Programming of Adult Diseases in Resource Poor Countries. Arch. Dis. Child. 2005, 90, 429–432. [Google Scholar] [CrossRef]
  10. Widdowson, E.M.; McCance, R.A. A Review: New Thoughts on Growth. Pediatr. Res. 1975, 9, 154–156. [Google Scholar] [CrossRef]
  11. Abu-Saad, K.; Fraser, D. Maternal Nutrition and Birth Outcomes. Epidemiol. Rev. 2010, 32, 5–25. [Google Scholar] [CrossRef]
  12. Wu, G.; Bazer, F.W.; Cudd, T.A.; Meininger, C.J.; Spencer, T.E. Maternal Nutrition and Fetal Development. J. Nutr. 2004, 134, 2169–2172. [Google Scholar] [CrossRef]
  13. Wu, G.; Bazer, F.W.; Wallace, J.M.; Spencer, T.E. Board-Invited Review: Intrauterine Growth Retardation: Implications for the Animal Sciences. J. Anim. Sci. 2006, 84, 2316–2337. [Google Scholar] [CrossRef]
  14. Innis, S.M. Influence of Maternal Cholestyramine Treatment on Cholesterol and Bile Acid Metabolism in Adult Offspring. J. Nutr. 1983, 113, 2464–2470. [Google Scholar] [CrossRef]
  15. Dicke, J.M.; Henderson, G.I. Placental Amino Acid Uptake in Normal and Complicated Pregnancies. Am. J. Med. Sci. 1988, 295, 223–227. [Google Scholar] [CrossRef] [PubMed]
  16. Stalker, L.A.; Ciminski, L.A.; Adams, D.C.; Klopfenstein, T.J.; Clark, R.T. Effects of Weaning Date and Prepartum Protein Supplementation on Cow Performance and Calf Growth. Rangel. Ecol. Manag. 2007, 60, 578–587. [Google Scholar] [CrossRef]
  17. Long, N.M.; Tousley, C.B.; Underwood, K.R.; Paisley, S.I.; Means, W.J.; Hess, B.W.; Du, M.; Ford, S.P. Effects of Early- to Mid-Gestational Undernutrition with or without Protein Supplementation on Offspring Growth, Carcass Characteristics, and Adipocyte Size in Beef Cattle. J. Anim. Sci. 2012, 90, 197–206. [Google Scholar] [CrossRef] [PubMed]
  18. Crouse, M.S.; Caton, J.S.; Cushman, R.A.; McLean, K.J.; Dahlen, C.R.; Borowicz, P.P.; Reynolds, L.P.; Ward, A.K. Moderate Nutrient Restriction of Beef Heifers Alters Expression of Genes Associated with Tissue Metabolism, Accretion, and Function in Fetal Liver, Muscle, and Cerebrum by Day 50 of Gestation. Transl. Anim. Sci. 2019, 3, 855–866. [Google Scholar] [CrossRef] [PubMed]
  19. Diniz, W.J.S.; Crouse, M.S.; Cushman, R.A.; McLean, K.J.; Caton, J.S.; Dahlen, C.R.; Reynolds, L.P.; Ward, A.K. Cerebrum, Liver, and Muscle Regulatory Networks Uncover Maternal Nutrition Effects in Developmental Programming of Beef Cattle during Early Pregnancy. Sci. Rep. 2021, 11, 2771. [Google Scholar] [CrossRef]
  20. Sulaiman, S.A.; de Blasio, M.J.; Harland, M.L.; Gatford, K.L.; Owens, J.A. Maternal Methyl Donor and Cofactor Supplementation in Late Pregnancy Increases β-Cell Numbers at 16 Days of Life in Growth-Restricted Twin Lambs. Am. J. Physiol. Endocrinol. Metab. 2017, 313, E381–E390. [Google Scholar] [CrossRef]
  21. Reynolds, L.P.; McLean, K.J.; McCarthy, K.L.; Diniz, W.J.S.; Menezes, A.C.B.; Forcherio, J.C.; Scott, R.R.; Borowicz, P.P.; Ward, A.K.; Dahlen, C.R.; et al. Nutritional Regulation of Embryonic Survival, Growth, and Development. Adv. Exp. Med. Biol. 2022, 1354, 63–76. [Google Scholar] [CrossRef]
  22. Foxcroft, G.R.; Dixon, W.T.; Novak, S.; Putman, C.T.; Town, S.C.; Vinsky, M.D. The Biological Basis for Prenatal Programming of Postnatal Performance in Pigs. J. Anim. Sci. 2006, 84, E105–E112. [Google Scholar] [CrossRef]
  23. Ji, Y.; Wu, Z.; Dai, Z.; Wang, X.; Li, J.; Wang, B.; Wu, G. Fetal and Neonatal Programming of Postnatal Growth and Feed Efficiency in Swine. J. Anim. Sci. Biotechnol. 2017, 8, 42. [Google Scholar] [CrossRef] [PubMed]
  24. Ford, S.P.; Long, N.M.; Ford, S.P.; Long, N.M. Evidence for Similar Changes in Offspring Phenotype Following Either Maternal Undernutrition or Overnutrition: Potential Impact on Fetal Epigenetic Mechanisms. Reprod. Fertil. Dev. 2011, 24, 105–111. [Google Scholar] [CrossRef] [PubMed]
  25. Funston, R.N.; Larson, D.M.; Vonnahme, K.A. Effects of Maternal Nutrition on Conceptus Growth and Offspring Performance: Implications for Beef Cattle Production. J. Anim. Sci. 2010, 88, E205–E215. [Google Scholar] [CrossRef] [PubMed]
  26. Wessels, I. Epigenetics and Minerals: An Overview. In Handbook of Nutrition, Diet, and Epigenetics; Springer: Berlin/Heidelberg, Germany, 2017. [Google Scholar]
  27. Harvey, K.M.; Fernandes Cooke, R.; Da, R.; Marques, S.; Paterson, M.; Relling, A.E. Supplementing Trace Minerals to Beef Cows during Gestation to Enhance Productive and Health Responses of the Offspring. Animals 2021, 11, 1159. [Google Scholar] [CrossRef]
  28. Dahlen, C.R.; Reynolds, L.P.; Caton, J.S. Selenium Supplementation and Pregnancy Outcomes. Front. Nutr. 2022, 9, 4715965. [Google Scholar] [CrossRef]
  29. Michels, K.B. Developmental Plasticity: Friend or Foe? Evol. Med. Public Health 2017, 2017, 183. [Google Scholar] [CrossRef] [PubMed]
  30. Sullivan, T.M.; Micke, G.; Greer, R.M.; Irving-Rodgers, H. Dietary Manipulation of Bos Indicus× Heifers during Gestation Affects the Reproductive Development of Their Heifer Calves. CSIRO Publ. 2009, 21, 773–784. [Google Scholar] [CrossRef]
  31. Ireland, J.J.; Smith, G.W.; Scheetz, D.; Jimenez-Krassel, F.; Folger, J.K.; Ireland, J.L.H.; Mossa, F.; Lonergan, P.; Evans, A.C.O. Does Size Matter in Females? An Overview of the Impact of the High Variation in the Ovarian Reserve on Ovarian Function and Fertility, Utility of Anti-Müllerian Hormone As. CSIRO Publ. 2011, 23, 1–14. [Google Scholar] [CrossRef]
  32. Roberts, A.J.; Petersen, M.K.; Funston, R.N. BEEF SPECIES SYMPOSIUM: Can We Build the Cowherd by Increasing Longevity of Females? J. Anim. Sci. 2015, 93, 4235–4243. [Google Scholar] [CrossRef]
  33. Patel, M.S.; Srinivasan, M. Metabolic Programming in the Immediate Postnatal Life. Ann. Nutr. Metab. 2011, 58, 18–28. [Google Scholar] [CrossRef] [PubMed]
  34. Dahlen, C.R.; Borowicz, P.P.; Ward, A.K.; Caton, J.S.; Czernik, M.; Palazzese, L.; Loi, P.; Reynolds, L.P. Programming of Embryonic Development. Int. J. Mol. Sci. 2021, 22, 1668. [Google Scholar] [CrossRef]
  35. Clara, A.; Menezes, B.; Dahlen, C.R.; Mccarthy, K.L.; Kassetas, C.J.; Baumgaertner, F.; Kirsch, J.D.; Dorsam, S.T.; Neville, T.L.; Ward, A.K.; et al. Fetal Hepatic Lipidome Is More Greatly Affected by Maternal Rate of Gain Compared with Vitamin and Mineral Supplementation at Day 83 of Gestation. Metabolites 2023, 13, 175. [Google Scholar] [CrossRef]
  36. Crouse, M.S.; McCarthy, K.L.; Menezes, A.C.B.; Kassetas, C.J.; Baumgaertner, F.; Kirsch, J.D.; Dorsam, S.; Neville, T.L.; Ward, A.K.; Borowicz, P.P.; et al. Vitamin and Mineral Supplementation and Rate of Weight Gain during the First Trimester of Gestation in Beef Heifers Alters the Fetal Liver Amino Acid, Carbohydrate, and Energy Profile at Day 83 of Gestation. Metabolites 2022, 12, 696. [Google Scholar] [CrossRef]
  37. Haggarty, P. Fatty Acid Supply to the Human Fetus. Annu. Rev. Nutr. 2010, 30, 237–255. [Google Scholar] [CrossRef] [PubMed]
  38. Martin, J.L.; Vonnahme, K.A.; Adams, D.C.; Lardy, G.P.; Funston, R.N. Effects of Dam Nutrition on Growth and Reproductive Performance of Heifer Calves. J. Anim. Sci. 2007, 85, 841–847. [Google Scholar] [CrossRef] [PubMed]
  39. Underwood, K.R.; Tong, J.F.; Price, P.L.; Roberts, A.J.; Grings, E.E.; Hess, B.W.; Means, W.J.; Du, M. Nutrition during Mid to Late Gestation Affects Growth, Adipose Tissue Deposition, and Tenderness in Cross-Bred Beef Steers. Meat Sci. 2010, 86, 588–593. [Google Scholar] [CrossRef]
  40. Wu, G.; Imhoff-Kunsch, B.; Girard, A.W. Biological Mechanisms for Nutritional Regulation of Maternal Health and Fetal Development. Paediatr. Perinat. Epidemiol. 2012, 26, 4–26. [Google Scholar] [CrossRef]
  41. Rasby, R.; Berger, A.; Bauer, D.; Brink, D. Minerals and Vitamins for Beef Cows; University of Nebraska-Lincoln: Lincoln, NE, USA, 2011. [Google Scholar]
  42. National Academies of Sciences, Engineering, and Medicine. Nutrient Requirements of Dairy Cattle, 8th revised ed.; National Academies Press: Washington, DC, USA, 2021. [Google Scholar] [CrossRef]
  43. National Academies of Sciences, Engineering, and Medicine. Nutrient Requirements of Beef Cattle, 8th revised ed.; National Academies Press: Washington, DC, USA, 2016. [Google Scholar]
  44. National Academies of Sciences, Engineering, and Medicine. Mineral Tolerance of Animals; National Academies Press: Washington, DC, USA, 2005. [Google Scholar]
  45. Warner, E.D. The Organogenesis and Early Histogenesis of the Bovine Stomach. Am. J. Anat. 1958, 102, 33–63. [Google Scholar] [CrossRef]
  46. Caton, J.S.; Crouse, M.S.; McLean, K.J.; Dahlen, C.R.; Ward, A.K.; Cushman, R.A.; Grazul-Bilska, A.T.; Neville, B.W.; Borowicz, P.P.; Reynolds, L.P. Maternal Periconceptual Nutrition, Early Pregnancy, and Developmental Outcomes in Beef Cattle. J. Anim. Sci. 2020, 98, skaa358. [Google Scholar] [CrossRef]
  47. Robinson, J.J.; Sinclair, K.D.; McEvoy, T.G. Nutritional Effects on Foetal Growth. Anim. Sci. 1999, 68, 315–331. [Google Scholar] [CrossRef]
  48. Diniz, W.J.S.; Crouse, M.S.; Caton, J.S.; Claycombe-Larson, K.J.; Lindholm-Perry, A.K.; Reynolds, L.P.; Dahlen, C.R.; Borowicz, P.P.; Ward, A.K. DNA Methylation Dataset of Bovine Embryonic Fibroblast Cells Treated with Epigenetic Modifiers and Divergent Energy Supply. Data Brief 2022, 42, 108074. [Google Scholar] [CrossRef]
  49. Crouse, M.S.; Caton, J.S.; Claycombe-Larson, K.J.; Diniz, W.J.S.; Lindholm-Perry, A.K.; Reynolds, L.P.; Dahlen, C.R.; Borowicz, P.P.; Ward, A.K. Epigenetic Modifier Supplementation Improves Mitochondrial Respiration and Growth Rates and Alters DNA Methylation of Bovine Embryonic Fibroblast Cells Cultured in Divergent Energy Supply. Front. Genet. 2022, 13, 812764. [Google Scholar] [CrossRef]
  50. Reynolds, L.P.; Ward, A.K.; Caton, J.S. Epigenetics and Developmental Programming in Ruminants: Long-Term Impacts on Growth and Development. In Biology of Domestic Animals; Taylor & Francis Group: Abingdon, UK, 2017; pp. 85–121. [Google Scholar] [CrossRef]
  51. Meyer, A.M.; Caton, J.S.; Hess, B.W.; Ford, S.P.; Reynolds, L.P. Epigenetics and Effects on the Neonate That May Impact Feed Efficiency. In Feed Efficiency in the Beef Industry; Wiley: Hoboken, NJ, USA, 2012; pp. 199–223. [Google Scholar] [CrossRef]
  52. Telford, N.A.; Watson, A.J.; Schultz, G.A. Transition from Maternal to Embryonic Control in Early Mammalian Development: A Comparison of Several Species. Mol. Reprod. Dev. 1990, 26, 90–100. [Google Scholar] [CrossRef]
  53. Peters, A.R. Embryo Mortality in the Cow. Anim. Breed. Abstr. 1996, 64, 587–598. [Google Scholar] [CrossRef]
  54. Flechon, J.E.; Renard, J.P. A Scanning Electron Microscope Study of the Hatching of Bovine Blastocysts in Vitro. J. Reprod. Fertil. 1978, 53, 9–12. [Google Scholar] [CrossRef] [PubMed]
  55. Shea, B.F. Evaluating the Bovine Embryo. Theriogenology 1981, 15, 31–42. [Google Scholar] [CrossRef] [PubMed]
  56. Russell, R.G.; Oteruelo, F.T. An Ultrastructural Study of the Differentiation of Skeletal Muscle in the Bovine Fetus. Anat. Embryol. 1981, 162, 403–417. [Google Scholar] [CrossRef]
  57. Winters, L.M.; Green, W.W.; Comstock, R.E. Prenatal Development of the Bovine; Agricultural Experiment Station: New Haven, CT, USA, 1942. [Google Scholar]
  58. Forde, N.; Beltman, M.E.; Duffy, G.B.; Duffy, P.; Mehta, J.P.; Ó’Gaora, P.; Roche, J.F.; Lonergan, P.; Crowe, M.A. Changes in the Endometrial Transcriptome During the Bovine Estrous Cycle: Effect of Low Circulating Progesterone and Consequences for Conceptus Elongation. Biol. Reprod. 2011, 84, 266–278. [Google Scholar] [CrossRef] [PubMed]
  59. Chen, M.; Dasgupta, C.; Xiong, F.; Zhang, L. Epigenetic Upregulation of Large-Conductance Ca2+- Activated K+ Channel Expression in Uterine Vascular Adaptation to Pregnancy. Hypertension 2014, 64, 610–618. [Google Scholar] [CrossRef]
  60. Bresnitz, W.; Lorca, R.A. Potassium Channels in the Uterine Vasculature: Role in Healthy and Complicated Pregnancies. Int. J. Mol. Sci. 2022, 23, 9446. [Google Scholar] [CrossRef] [PubMed]
  61. Nagar, D.; Liu, X.T.; Rosenfeld, C.R. Estrogen Regulates Β1-Subunit Expression in Ca 2+-Activated K+ Channels in Arteries from Reproductive Tissues. Am. J. Physiol. Heart Circ. Physiol. 2005, 289, 1417–1427. [Google Scholar] [CrossRef] [PubMed]
  62. Veiga, G.A.L.; Milazzotto, M.P.; Nichi, M.; Lúcio, C.F.; Silva, L.C.G.; Angrimani, D.S.R.; Vannucchi, C.I. Gene Expression of Estrogen and Oxytocin Receptors in the Uterus of Pregnant and Parturient Bitches. Braz. J. Med. Biol. Res. 2015, 48, 339–343. [Google Scholar] [CrossRef]
  63. Magness, R.R. Maternal Cardiovascular and Other Physiologic Responses to the Endocrinology of Pregnancy. In Endocrinology of Pregnancy; Springer: Berlin/Heidelberg, Germany, 1998; pp. 507–539. [Google Scholar] [CrossRef]
  64. Reynolds, L.P.; Borowicz, P.P.; Caton, J.S.; Vonnahme, K.A.; Luther, J.S.; Buchanan, D.S.; Hafez, S.A.; Grazul-Bilska, A.T.; Redmer, D.A. Uteroplacental Vascular Development and Placental Function: An Update. Int. J. Dev. Biol. 2010, 54, 355–365. [Google Scholar] [CrossRef]
  65. Goff, J.P. Invited Review: Mineral Absorption Mechanisms, Mineral Interactions That Affect Acid-Base and Antioxidant Status, and Diet Considerations to Improve Mineral Status. J. Dairy Sci. 2018, 101, 2763–2813. [Google Scholar] [CrossRef] [PubMed]
  66. Keen, C.L. Teratogenic Effects of Essential Trace Metals: Deficiency and Excesses. In Toxicology of Metals; Chang, L.W., Magos, L., Suzuki, T., Eds.; Academic Press: Cambridge, MA, USA, 1996; pp. 977–1001. [Google Scholar]
  67. Rogers, J.M.; Keen, C.L.; Hurley, L.S. Zinc Deficiency in Pregnant Long-Evans Hooded Rats: Teratogenicity and Tissue Trace Elements. Teratology 1985, 31, 89–100. [Google Scholar] [CrossRef] [PubMed]
  68. Ma, J.; Zhao, N.; Zhu, D. Bioabsorbable Zinc Ion Induced Biphasic Cellular Responses in Vascular Smooth Muscle Cells. Sci. Rep. 2016, 6, 26661. [Google Scholar] [CrossRef] [PubMed]
  69. Zong, L.; Wei, X.; Gou, W.; Huang, P.; Lv, Y. Zinc Improves Learning and Memory Abilities of Fetal Growth Restriction Rats and Promotes Trophoblast Cell Invasion and Migration via Enhancing STAT3-MMP-2/9 Axis Activity. Oncotarget 2017, 8, 115190. [Google Scholar] [CrossRef]
  70. Aruga, J.; Millen, K.J. ZIC1 Function in Normal Cerebellar Development and Human Developmental Pathology. Adv. Exp. Med. Biol. 2018, 1046, 249–268. [Google Scholar] [CrossRef]
  71. Aruga, J.; Nozaki, Y.; Hatayama, M.; Odaka, Y.S.; Yokota, N. Expression of ZIC Family Genes in Meningiomas and Other Brain Tumors. BMC Cancer 2010, 10, 79. [Google Scholar] [CrossRef]
  72. Aruga, J.; Inoue, T.; Hoshino, J.; Mikoshiba, K. Zic2 Controls Cerebellar Development in Cooperation with Zic1. J. Neurosci. 2002, 22, 218–225. [Google Scholar] [CrossRef]
  73. Cho, H.J.; Park, J.H.; Nam, J.H.; Chang, Y.C.; Park, B.; Hoe, H.S. Ascochlorin Suppresses MMP-2-Mediated Migration and Invasion by Targeting FAK and JAK-STAT Signaling Cascades. J. Cell. Biochem. 2018, 119, 300–313. [Google Scholar] [CrossRef]
  74. Lopez, V.; Keen, C.L.; Lanoue, L. Prenatal Zinc Deficiency: Influence on Heart Morphology and Distribution of Key Heart Proteins in a Rat Model. Biol. Trace Elem. Res. 2008, 122, 238–255. [Google Scholar] [CrossRef] [PubMed]
  75. Tian, X.; Zheng, Y.; Li, Y.; Shen, Z.; Tao, L.; Dou, X.; Qian, J.; Shen, H. Psychological Stress Induced Zinc Accumulation and Up-Regulation of ZIP14 and Metallothionein in Rat Liver. BMC Gastroenterol. 2014, 14, 32. [Google Scholar] [CrossRef]
  76. Bennetts, H.W.; Chapman, F.E. Copper Deficiency in Sheep in Western Australia: A Preliminary Account of the Ætiology of Enzootic Ataxia of Lambs and an Anæmia of Ewes. Aust. Vet. J. 1937, 13, 138–149. [Google Scholar] [CrossRef]
  77. Harvey, K.M.; Cooke, R.F.; Colombo, E.A.; Rett, B.; de Sousa, O.A.; Harvey, L.M.; Russell, J.R.; Pohler, K.G.; Brandão, A.P. Supplementing Organic-Complexed or Inorganic Co, Cu, Mn, and Zn to Beef Cows during Gestation: Physiological and Productive Response of Cows and Their Offspring until Weaning. J. Anim. Sci. 2021, 99, skab095. [Google Scholar] [CrossRef] [PubMed]
  78. Gould, L.; Kendall, N.R. Role of the Rumen in Copper and Thiomolybdate Absorption. Nutr. Res. Rev. 2011, 24, 176. [Google Scholar] [CrossRef] [PubMed]
  79. Mills, C.F.; Williams, R.B. Copper Concentration and Cytochrome-Oxidase and Ribonuclease Activities in the Brains of Copper-Deficient Lambs. Biochem. J. 1962, 85, 629–632. [Google Scholar] [CrossRef]
  80. Williams, J.R.; Trias, E.; Beilby, P.R.; Lopez, N.I.; Labut, E.M.; Bradford, C.S.; Roberts, B.R.; McAllum, E.J.; Crouch, P.J.; Rhoads, T.W.; et al. Copper Delivery to the CNS by CuATSM Effectively Treats Motor Neuron Disease in SODG93A Mice Co-Expressing the Copper-Chaperone-for-SOD. Neurobiol. Dis. 2016, 89, 1–9. [Google Scholar] [CrossRef]
  81. Choi, J.; Rees, H.D.; Weintraub, S.T.; Levey, A.I.; Chin, L.S.; Li, L. Oxidative Modifications and Aggregation of Cu,Zn-Superoxide Dismutase Associated with Alzheimer and Parkinson Diseases. J. Biol. Chem. 2005, 280, 11648–11655. [Google Scholar] [CrossRef]
  82. Lei, X.G.; Combs, G.F.; Sunde, R.A.; Caton, J.S.; Arthington, J.D.; Vatamaniuk, M.Z. Dietary Selenium Across Species. Annu. Rev. Nutr. 2022, 42, 337–375. [Google Scholar] [CrossRef] [PubMed]
  83. Diniz, W.J.S.; Bobe, G.; Ward, A.K.; Hall, J.A.; Klopfenstein, J.J.; Gultekin, Y.; Davis, T.Z. Supranutritional Maternal Organic Selenium Supplementation during Different Trimesters of Pregnancy Affects the Muscle Gene Transcriptome of Newborn Beef Calves in a Time-Dependent Manner. Genes 2021, 12, 1884. [Google Scholar] [CrossRef] [PubMed]
  84. Qazi, I.H.; Angel, C.; Yang, H.; Pan, B.; Zoidis, E.; Zeng, C.J.; Han, H.; Zhou, G. bin Selenium, Selenoproteins, and Female Reproduction: A Review. Molecules 2018, 23, 3053. [Google Scholar] [CrossRef] [PubMed]
  85. Ojeda, M.L.; Nogales, F.; Romero-Herrera, I.; Carreras, O. Fetal Programming Is Deeply Related to Maternal Selenium Status and Oxidative Balance; Experimental Offspring Health Repercussions. Nutrients 2021, 13, 2085. [Google Scholar] [CrossRef]
  86. Ojeda, M.L.; Carreras, O.; Díaz-Castro, J.; Murillo, M.L.; Nogales, F. High- and Low- Selenium Diets Affect Endocrine Energy Balance during Early Programming. Toxicol. Appl. Pharmacol. 2019, 382, 114744. [Google Scholar] [CrossRef] [PubMed]
  87. Arthur, J.R.; Nicol, F.; Hutchinson, A.R.; Beckett, G.J. The Effects of Selenium Depletion and Repletion on the Metabolism of Thyroid Hormones in the Rat. J. Inorg. Biochem. 1990, 39, 101–108. [Google Scholar] [CrossRef]
  88. Ward, M.A.; Neville, T.L.; Reed, J.J.; Taylor, J.B.; Hallford, D.M.; Soto-Navarro, S.A.; Vonnahme, K.A.; Redmer, D.A.; Reynolds, L.P.; Caton, J.S. Effects of Selenium Supply and Dietary Restriction on Maternal and Fetal Metabolic Hormones in Pregnant Ewe Lambs. J. Anim. Sci. 2008, 86, 1254–1262. [Google Scholar] [CrossRef]
  89. Kang, D.; Lee, J.; Wu, C.; Guo, X.; Lee, B.J.; Chun, J.S.; Kim, J.H. The Role of Selenium Metabolism and Selenoproteins in Cartilage Homeostasis and Arthropathies. Exp. Mol. Med. 2020, 52, 1198–1208. [Google Scholar] [CrossRef]
  90. Pappas, A.C.; Zoidis, E.; Chadio, S.E. Maternal Selenium and Developmental Programming. Antioxidants 2019, 8, 145. [Google Scholar] [CrossRef]
  91. Arthur, J.R.; Beckett, G.J.; Mitchell, J.H.; Arthur, J. The Interactions between Selenium and Iodine Deficiencies in Man and Animals. Nutr. Res. Rev. 1999, 12, 55–73. [Google Scholar] [CrossRef]
  92. Abuid, J.; Stinson, D.A.; Larsen, P.R. Serum Triiodothyronine and Thyroxine in the Neonate and the Acute Increases in These Hormones Following Delivery. J. Clin. Investig. 1973, 52, 1195–1199. [Google Scholar] [CrossRef]
  93. Dellavalle, A.; Maroli, G.; Covarello, D.; Azzoni, E.; Innocenzi, A.; Perani, L.; Antonini, S.; Sambasivan, R.; Brunelli, S.; Tajbakhsh, S.; et al. Pericytes Resident in Postnatal Skeletal Muscle Differentiate into Muscle Fibres and Generate Satellite Cells. Nat. Commun. 2011, 2, 499. [Google Scholar] [CrossRef] [PubMed]
  94. Du, M.; Tong, J.; Zhao, J.; Underwood, K.R.; Zhu, M.; Ford, S.P.; Nathanielsz, P.W. Fetal Programming of Skeletal Muscle Development in Ruminant Animals. J. Anim. Sci. 2010, 88, E51–E60. [Google Scholar] [CrossRef] [PubMed]
  95. Brent, G.A. Mechanisms of Thyroid Hormone Action. J. Clin. Investig. 2012, 122, 3035–3043. [Google Scholar] [CrossRef]
  96. Yu, F.; Göthe, S.; Wikström, L.; Forrest, D.; Vennström, B.; Larsson, L. Effects of Thyroid Hormone Receptor Gene Disruption on Myosin Isoform Expression in Mouse Skeletal Muscles. Am. J. Physiol. Regul. Integr. Comp. Physiol. 2000, 278, R1545–R1554. [Google Scholar] [CrossRef]
  97. Cheng, S.Y.; Leonard, J.L.; Davis, P.J. Molecular Aspects of Thyroid Hormone Actions. Endocr. Rev. 2010, 31, 139–170. [Google Scholar] [CrossRef] [PubMed]
  98. Hiroi, Y.; Kim, H.H.; Ying, H.; Furuya, F.; Huang, Z.; Simoncini, T.; Noma, K.; Ueki, K.; Nguyen, N.H.; Scanlan, T.S.; et al. Rapid Nongenomic Actions of Thyroid Hormone. Proc. Natl. Acad. Sci. USA 2006, 103, 14104–14109. [Google Scholar] [CrossRef]
  99. Tomanek, R.J.; Zimmerman, M.B.; Suvarna, P.R.; Morkin, E.; Pennock, G.D.; Goldman, S. A Thyroid Hormone Analog Stimulates Angiogenesis in the Post-Infarcted Rat Heart. J. Mol. Cell. Cardiol. 1998, 30, 923–932. [Google Scholar] [CrossRef] [PubMed]
  100. Zimmermann, M.B.; Köhrle, J. The Impact of Iron and Selenium Deficiencies on Iodine and Thyroid Metabolism: Biochemistry and Relevance to Public Health. Thyroid 2002, 12, 867–878. [Google Scholar] [CrossRef]
  101. Goyens, P.; Golstein, J.; Nsombola, B.; Vis, H.; Dumont, J.E. Selenium Deficiency as a Possible Factor in the Pathogenesis of Myxoedematous Endemic Cretinism. Eur. J. Endocrinol. 1987, 114, 497–502. [Google Scholar] [CrossRef]
  102. Maxwell, C.; Volpe, S.L. Effect of Zinc Supplementation on Thyroid Hormone Function. Ann. Nutr. Metab. 2007, 51, 188–194. [Google Scholar] [CrossRef] [PubMed]
  103. Hess, S.Y.; Zimmermann, M.B.; Arnold, M.; Langhans, W.; Hurrell, R.F. Iron Deficiency Anemia Reduces Thyroid Peroxidase Activity in Rats. J. Nutr. 2002, 132, 1951–1955. [Google Scholar] [CrossRef] [PubMed]
  104. Vinayagamoorthi, R.; Dhiman, P.; Kollipaka, R.; Sabita, P.; Hemavathy, V. Association of Hypothyroidism with Low Serum Ferritin Levels and Iron-Deficiency Anemia During the First Trimester of Pregnancy. Cureus 2022, 14, e28307. [Google Scholar] [CrossRef]
  105. Kovacs, C.S.; Ho-Pao, C.L.; Hunzelman, J.L.; Lanske, B.; Fox, J.; Seidman, J.G.; Seidman, C.E.; Kronenberg, H.M. Regulation of Murine Fetal-Placental Calcium Metabolism by the Calcium-Sensing Receptor. J. Clin. Investig. 1998, 101, 2812–2820. [Google Scholar] [CrossRef]
  106. Lofrese, J.J.; Basit, H.; Lappin, S.L. Physiology, Parathyroid; StatPearls: Thousand Oaks, CA, USA, 2022. [Google Scholar]
  107. Castiglioni, S.; Cazzaniga, A.; Albisetti, W.; Maier, J.A.M. Magnesium and Osteoporosis: Current State of Knowledge and Future Research Directions. Nutrients 2013, 5, 3022–3033. [Google Scholar] [CrossRef]
  108. Malucelli, E.; Guidetti, M.; Orsola-Malpighi, P.S.; Farruggia, G.; Pinna, A.D. The Complex Relationship between Magnesium and Serum Parathyroid Hormone: A Study in Patients with Chronic Intestinal Failure I Go MILS-Italian Group of Minimally Invasive Liver Surgery View Project Liver Transplantation View Project; John Libbey Eurotext Limited: Arcueil, France, 2009. [Google Scholar] [CrossRef]
  109. White, A.D.; Peña, K.A.; Clark, L.J.; Maria, C.S.; Liu, S.; Jean-Alphonse, F.G.; Lee, J.Y.; Lei, S.; Cheng, Z.; Tu, C.-L.; et al. Spatial Bias in CAMP Generation Determines Biological Responses to PTH Type 1 Receptor Activation. Sci. Signal. 2021, 14, eabc5944. [Google Scholar] [CrossRef]
  110. Lombardi, G.; Ziemann, E.; Banfi, G.; Corbetta, S. Physical Activity-Dependent Regulation of Parathyroid Hormone and Calcium-Phosphorous Metabolism. Int. J. Mol. Sci. 2020, 21, 5388. [Google Scholar] [CrossRef]
  111. Khan, A.A.; Clarke, B.; Rejnmark, L.; Brandi, M.L. Management of Endocrine Disease: Hypoparathyroidism in Pregnancy: Review and Evidence-Based Recommendations for Management. Eur. J. Endocrinol. 2019, 180, R37–R44. [Google Scholar] [CrossRef]
  112. Li, P.; Chang, X.; Fan, X.; Fan, C.; Tang, T.; Wang, R.; Qi, K. Dietary Calcium Status during Maternal Pregnancy and Lactation Affects Lipid Metabolism in Mouse Offspring. Sci. Rep. 2018, 8, 16542. [Google Scholar] [CrossRef]
  113. Ellinger, I. The Calcium-Sensing Receptor and the Reproductive System. Front. Physiol. 2016, 7, 371. [Google Scholar] [CrossRef]
  114. McCarthy, K.L.; Ana, A.C.; Kassetas, C.J.; Baumgaertner, F.; Kirsch, J.D.; Dorsam, S.T.; Neville, T.L.; Ward, A.K.; Borowicz, P.P.; Reynolds, L.P.; et al. Vitamin and Mineral Supplementation and Rate of Gain in Beef Heifers II: Effects on Concentration of Trace Minerals in Maternal Liver and Fetal Liver, Muscle, Allantoic, and Amniotic Fluids at Day 83 of Gestation. Animals 2022, 12, 1925. [Google Scholar] [CrossRef] [PubMed]
  115. Menezes, A.C.B.; McCarthy, K.L.; Kassetas, C.J.; Baumgaertner, F.; Kirsch, J.D.; Dorsam, S.T.; Neville, T.L.; Ward, A.K.; Borowicz, P.P.; Reynolds, L.P.; et al. Vitamin and Mineral Supplementation and Rate of Gain in Beef Heifers I: Effects on Dam Hormonal and Metabolic Status, Fetal Tissue and Organ Mass, and Concentration of Glucose and Fructose in Fetal Fluids at d 83 of Gestation. Animals 2022, 12, 1757. [Google Scholar] [CrossRef]
  116. Diniz, W.J.S.; Reynolds, L.P.; Borowicz, P.P.; Ward, A.K.; Sedivec, K.K.; McCarthy, K.L.; Kassetas, C.J.; Baumgaertner, F.; Kirsch, J.D.; Dorsam, S.T.; et al. Maternal Vitamin and Mineral Supplementation and Rate of Maternal Weight Gain Affects Placental Expression of Energy Metabolism and Transport-Related Genes. Genes 2021, 12, 385. [Google Scholar] [CrossRef] [PubMed]
  117. Diniz, W.J.S.; Ward, A.K.; Mccarthy, K.L.; Kassetas, C.J.; Baumgaertner, F.; Reynolds, L.P.; Borowicz, P.P.; Sedivec, K.K.; Kirsch, J.D.; Dorsam, S.T.; et al. Periconceptual Maternal Nutrition Affects Fetal Liver Programming of Energy- and Lipid-Related Genes. Animals 2023, 13, 600. [Google Scholar] [CrossRef]
  118. Anagnostis, P.; Athyros, V.G.; Tziomalos, K.; Karagiannis, A.; Mikhailidis, D.P. The Pathogenetic Role of Cortisol in the Metabolic Syndrome: A Hypothesis. J. Clin. Endocrinol. Metab. 2009, 94, 2692–2701. [Google Scholar] [CrossRef] [PubMed]
  119. Takaya, J.; Iharada, A.; Okihana, H.; Kaneko, K. Magnesium Deficiency in Pregnant Rats Alters Methylation of Specific Cytosines in the Hepatic Hydroxysteroid Dehydrogenase-2 Promoter of the Offspring View Supplementary Material. Epigenetics 2011, 6, 573–578. [Google Scholar] [CrossRef]
  120. Tran, P.V.; Kennedy, B.C.; Lien, Y.C.; Simmons, R.A.; Georgieff, M.K. Fetal Iron Deficiency Induces Chromatin Remodeling at the Bdnf Locus in Adult Rat Hippocampus. Am. J. Physiol. Regul. Integr. Comp. Physiol. 2015, 308, R276–R282. [Google Scholar] [CrossRef]
  121. Lien, Y.C.; Condon, D.E.; Georgieff, M.K.; Simmons, R.A.; Tran, P.V. Dysregulation of Neuronal Genes by Fetal-Neonatal Iron Deficiency Anemia Is Associated with Altered DNA Methylation in the Rat Hippocampus. Nutrients 2019, 11, 1191. [Google Scholar] [CrossRef]
  122. Schachtschneider, K.M.; Liu, Y.; Rund, L.A.; Madsen, O.; Johnson, R.W.; Groenen, M.A.M.; Schook, L.B. Impact of Neonatal Iron Deficiency on Hippocampal DNA Methylation and Gene Transcription in a Porcine Biomedical Model of Cognitive Development. BMC Genom. 2016, 17, 856. [Google Scholar] [CrossRef]
  123. Kurita, H.; Ohsako, S.; Hashimoto, S.-I.; Yoshinaga, J.; Tohyama, C. Prenatal Zinc Deficiency-Dependent Epigenetic Alterations of Mouse Metallothionein-2 Gene. J. Nutr. Biochem. 2013, 24, 256–266. [Google Scholar] [CrossRef]
  124. Wischhusen, P.; Saito, T.; Heraud, C.; Kaushik, S.J.; Fauconneau, B.; Prabhu, P.A.J.; Fontagné-Dicharry, S.; Skjӕrven, K.H. Parental Selenium Nutrition Affects the One-Carbon Metabolism and the Hepatic DNA Methylation Pattern of Rainbow Trout (Oncorhynchus Mykiss) in the Progeny. Life 2020, 10, 121. [Google Scholar] [CrossRef] [PubMed]
  125. Kennedy, E.; Everson, T.M.; Punshon, T.; Jackson, B.P.; Hao, K.; Lambertini, L.; Chen, J.; Karagas, M.R.; Marsit, C.J. Copper Associates with Differential Methylation in Placentae from Two US Birth Cohorts. Epigenetics 2020, 15, 215. [Google Scholar] [CrossRef] [PubMed]
  126. Espart, A.; Artime, S.; Tort-Nasarre, G.; Yara-Varón, E. Cadmium Exposure during Pregnancy and Lactation: Materno-Fetal and Newborn Repercussions of Cd(Ii), and Cd–Metallothionein Complexes. Metallomics 2018, 10, 1359–1367. [Google Scholar] [CrossRef] [PubMed]
  127. Sekovanić, A.; Jurasović, J.; Piasek, M. Metallothionein 2A Gene Polymorphisms in Relation to Diseases and Trace Element Levels in Humans. Arch. Ind. Hyg. Toxicol. 2020, 71, 27. [Google Scholar] [CrossRef]
  128. Zheng, D.; Feeney, G.P.; Kille, P.; Hogstrand, C. Regulation of ZIP and ZnT Zinc Transporters in Zebrafish Gill: Zinc Repression of ZIP10 Transcription by an Intronic MRE Cluster. Physiol. Genom. 2008, 34, 205–214. [Google Scholar] [CrossRef] [PubMed]
  129. Yamaji, S.; Tennant, J.; Tandy, S.; Williams, M.; Singh Srai, S.K.; Sharp, P. Zinc Regulates the Function and Expression of the Iron Transporters DMT1 and IREG1 in Human Intestinal Caco-2 Cells. FEBS Lett. 2001, 507, 137–141. [Google Scholar] [CrossRef]
  130. Davis, C.D.; Uthus, E.O.; Finley, J.W. Dietary Selenium and Arsenic Affect DNA Methylation In Vitro in Caco-2 Cells and In Vivo in Rat Liver and Colon. J. Nutr. 2000, 130, 2903–2909. [Google Scholar] [CrossRef]
  131. Uthus, E.O.; Ross, S.A.; Davis, C.D. Differential Effects of Dietary Selenium (Se) and Folate on Methyl Metabolism in Liver and Colon of Rats. Biol. Trace Elem. Res. 2006, 109, 201–214. [Google Scholar] [CrossRef]
  132. Davis, C.D.; Uthus, E.O. Dietary Selenite and Azadeoxycytidine Treatments Affect Dimethylhydrazine-Induced Aberrant Crypt Formation in Rat Colon and DNA Methylation in HT-29 Cells. J. Nutr. 2002, 132, 292–297. [Google Scholar] [CrossRef]
  133. Davis, C.D.; Uthus, E.O. Dietary Folate and Selenium Affect Dimethylhydrazine-Induced Aberrant Crypt Formation, Global DNA Methylation and One-Carbon Metabolism in Rats. J. Nutr. 2003, 133, 2907–2914. [Google Scholar] [CrossRef]
  134. Frazer, D.M.; Wilkins, S.J.; Becker, E.M.; Murphy, T.L.; Vulpe, C.D.; McKie, A.T.; Anderson, G.J. A Rapid Decrease in the Expression of DMT1 and Dcytb but Not Ireg1 or Hephaestin Explains the Mucosal Block Phenomenon of Iron Absorption. Gut 2003, 52, 340. [Google Scholar] [CrossRef] [PubMed]
  135. Michaelis, V.; Aengenheister, L.; Tuchtenhagen, M.; Rinklebe, J.; Ebert, F.; Schwerdtle, T.; Buerki-Thurnherr, T.; Bornhorst, J. Differences and Interactions in Placental Manganese and Iron Transfer across an In Vitro Model of Human Villous Trophoblasts. Int. J. Mol. Sci. 2022, 23, 3296. [Google Scholar] [CrossRef]
  136. Arredondo, M.; Muñoz, P.; Mura, C.V.; Núñez, M.T. DMT1, a Physiologically Relevant Apical Cu1+ Transporter of Intestinal Cells. Am. J. Physiol. Cell. Physiol. 2003, 284, C1525–C1530. [Google Scholar] [CrossRef] [PubMed]
  137. Gruper, Y.; Bar, J.; Bacharach, E.; Ehrlich, R. Transferrin Receptor Co-Localizes and Interacts with the Hemochromatosis Factor (HFE) and the Divalent Metal Transporter-1 (DMT1) in Trophoblast Cells. J. Cell. Physiol. 2005, 204, 901–912. [Google Scholar] [CrossRef]
  138. Hardman, B.; Manuelpillai, U.; Wallace, E.M.; van de Waasenburg, S.; Cater, M.; Mercer, J.F.B.; Ackland, M.L. Expression and Localization of Menkes and Wilson Copper Transporting ATPases in Human Placenta. Placenta 2004, 25, 512–517. [Google Scholar] [CrossRef] [PubMed]
  139. McArdle, H.J.; Andersen, H.S.; Jones, H.; Gambling, L. Copper and Iron Transport Across the Placenta: Regulation and Interactions. J. Neuroendocrinol. 2008, 20, 427–431. [Google Scholar] [CrossRef]
  140. Takaya, J. Calcium-Deficiency during Pregnancy Affects Insulin Resistance in Offspring. Int. J. Mol. Sci. 2021, 22, 7008. [Google Scholar] [CrossRef]
  141. Takaya, J.; Yamanouchi, S.; Tanabe, Y.; Kaneko, K. A Calcium-Deficient Diet in Rat Dams during Gestation Decreases HOMA-Β% in 3 Generations of Offspring. J. Nutrigenet. Nutr. 2017, 9, 276–286. [Google Scholar] [CrossRef]
  142. Gao, H.; Wu, G.; Spencer, T.E.; Johnson, G.A.; Li, X.; Bazer, F.W. Select Nutrients in the Ovine Uterine Lumen. I. Amino Acids, Glucose, and Ions in Uterine Lumenal Flushings of Cyclic and Pregnant Ewes. Biol. Reprod. 2009, 80, 86–93. [Google Scholar] [CrossRef]
  143. McArdle, H.J.; Douglas, A.J.; Morgan, E.H. Transferrin Binding by Microvillar Vesicles Isolated from Rat Placenta. Placenta 1984, 5, 131–138. [Google Scholar] [CrossRef]
  144. Srai, S.K.S.; Bomford, A.; McArdle, H.J. Iron Transport across Cell Membranes: Molecular Understanding of Duodenal and Placental Iron Uptake. Best Pract. Res. Clin. Haematol. 2002, 15, 243–259. [Google Scholar] [CrossRef]
  145. Lee, J.; Prohaska, J.R.; Thiele, D.J. Essential Role for Mammalian Copper Transporter Ctr1 in Copper Homeostasis and Embryonic Development. Proc. Natl. Acad. Sci. USA 2001, 98, 6842–6847. [Google Scholar] [CrossRef] [PubMed]
  146. Han, H.; Archibeque, S.L.; Engle, T.E. Characterization and Identification of Hepatic MRNA Related to Copper Metabolism and Homeostasis in Cattle. Biol. Trace Elem. Res. 2009, 129, 130–136. [Google Scholar] [CrossRef] [PubMed]
  147. Khayat, S.; Fanaei, H.; Ghanbarzehi, A. Minerals in Pregnancy and Lactation: A Review Article. J. Clin. Diagn. Res. 2017, 11, QE01. [Google Scholar] [CrossRef]
  148. Phillips, N.L.H.; Roth, T.L. Animal Models and Their Contribution to Our Understanding of the Relationship Between Environments, Epigenetic Modifications, and Behavior. Genes 2019, 10, 47. [Google Scholar] [CrossRef] [PubMed]
  149. Reynolds, L.P.; Vonnahme, K.A. Livestock as Models for Developmental Programming. Anim. Front. 2017, 7, 12–17. [Google Scholar] [CrossRef]
  150. Armitage, J.A.; Khan, I.Y.; Taylor, P.D.; Nathanielsz, P.W.; Poston, L. Developmental Programming of the Metabolic Syndrome by Maternal Nutritional Imbalance: How Strong Is the Evidence from Experimental Models in Mammals? J. Physiol. 2004, 561, 355–377. [Google Scholar] [CrossRef]
  151. Fitz-James, M.H.; Cavalli, G. Molecular Mechanisms of Transgenerational Epigenetic Inheritance. Nat. Rev. Genet. 2022, 23, 325–341. [Google Scholar] [CrossRef]
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Figure 1. Timeline indicating organogenesis and development of different structures during gestation in cattle [45,46,52,53,54,55,56,57,58].
Figure 1. Timeline indicating organogenesis and development of different structures during gestation in cattle [45,46,52,53,54,55,56,57,58].
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Figure 2. Schematic overview of the role of estrogen, Ca+2, and K+ in the establishment of pregnancy-associated relaxation and myogenic tone reduction. Pregnancy increases the basal estrogen level and demethylate CpG at the Sp1 promotor site to increase KCNMB1 expression [61]. KCNMB1 leads to opening of BKca channels, causing efflux of K+ and release of Ca+2, which further promote KCNMB1 expression [59]. Change in membrane potential of vascular smooth muscle in the uterine artery by efflux of K+ and release of Ca+2 results in uterine artery dilation along with pregnancy-induced relaxation [61]. KCNMB1, potassium calcium-activated channel subfamily M regulatory Beta subunit 1; BKCa, large-conductance Ca+2-activated K+ channel receptors.
Figure 2. Schematic overview of the role of estrogen, Ca+2, and K+ in the establishment of pregnancy-associated relaxation and myogenic tone reduction. Pregnancy increases the basal estrogen level and demethylate CpG at the Sp1 promotor site to increase KCNMB1 expression [61]. KCNMB1 leads to opening of BKca channels, causing efflux of K+ and release of Ca+2, which further promote KCNMB1 expression [59]. Change in membrane potential of vascular smooth muscle in the uterine artery by efflux of K+ and release of Ca+2 results in uterine artery dilation along with pregnancy-induced relaxation [61]. KCNMB1, potassium calcium-activated channel subfamily M regulatory Beta subunit 1; BKCa, large-conductance Ca+2-activated K+ channel receptors.
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Figure 3. Proposed mechanism of fetal–maternal transport of selenium and iodine and their role in thyroxine metabolism in cattle. Maternal selenium concentration impacts the expression of selenoproteins, i.e., SEPP1 and Dio2 in dam’s liver [89]. SEPP1 will be transported to fetus by ApoER2, and Dio2 will affect thyroxines interconversion across fetal–maternal tissues [85,89,90,91,92]. SEPSECS, (Sep (O-Phosphoserine) TRNA:Sec (Selenocysteine) TRNA Synthase); SBP2, selenocysteine binding protein 2; SEPP1, Selenoprotein-P; Dio2, TypeII Deiodinase; ApoER2, Apolipoprotein E Receptor-2; Dio3, TypeIII Deiodinase; T3, Triiodothyronine-3; T4, Thyroxine-4.
Figure 3. Proposed mechanism of fetal–maternal transport of selenium and iodine and their role in thyroxine metabolism in cattle. Maternal selenium concentration impacts the expression of selenoproteins, i.e., SEPP1 and Dio2 in dam’s liver [89]. SEPP1 will be transported to fetus by ApoER2, and Dio2 will affect thyroxines interconversion across fetal–maternal tissues [85,89,90,91,92]. SEPSECS, (Sep (O-Phosphoserine) TRNA:Sec (Selenocysteine) TRNA Synthase); SBP2, selenocysteine binding protein 2; SEPP1, Selenoprotein-P; Dio2, TypeII Deiodinase; ApoER2, Apolipoprotein E Receptor-2; Dio3, TypeIII Deiodinase; T3, Triiodothyronine-3; T4, Thyroxine-4.
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Figure 4. Proposed mechanism of feto-maternal transport of Ca, P, Mg, and iodine and their roles in regulating molecular mechanism of parathyroid hormone (PTH) and calcitriol (1,25-dihydroxycholecalciferol, 1,25(OH)2D) in cattle. Maternal Ca+2 concentration causes a change in the expression of PTHrP in placenta and mammary tissue along with the expression of CaSR in placenta [105,111,113]. PTH is regulated by CaSR in the fetus and maternal PTHrP binds to PTHR1 in the kidney and activates the cAMP-associated conversion of calcitriol (1,25(OH)D), in which Mg+2 will be used as a cofactor [109,110,111]. CaSR, calcium sensing receptor; PTHrP, parathyroid hormone related proteins; PTHR1, parathyroid hormone 1 receptor; cAMP, cyclic adenosine monophosphate; PKA, phosphokinase activated; CREB, cAMP response element-binding protein; calcitriol, 1,25(OH)D.
Figure 4. Proposed mechanism of feto-maternal transport of Ca, P, Mg, and iodine and their roles in regulating molecular mechanism of parathyroid hormone (PTH) and calcitriol (1,25-dihydroxycholecalciferol, 1,25(OH)2D) in cattle. Maternal Ca+2 concentration causes a change in the expression of PTHrP in placenta and mammary tissue along with the expression of CaSR in placenta [105,111,113]. PTH is regulated by CaSR in the fetus and maternal PTHrP binds to PTHR1 in the kidney and activates the cAMP-associated conversion of calcitriol (1,25(OH)D), in which Mg+2 will be used as a cofactor [109,110,111]. CaSR, calcium sensing receptor; PTHrP, parathyroid hormone related proteins; PTHR1, parathyroid hormone 1 receptor; cAMP, cyclic adenosine monophosphate; PKA, phosphokinase activated; CREB, cAMP response element-binding protein; calcitriol, 1,25(OH)D.
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Figure 5. Proposed mechanism of fetomaternal transport of Fe, Mn, Zn, and Cu in cattle. Iron or manganese can form complexes with transferrin and bind to TfR1 in the placenta, which transports Fe or Mn to the fetus [135,137]. Cu and Zn are also transported by placental transporters CTR1 or Cu-Zn SOD [77,81,138,139] and ZIP14 [75], respectively. All these mentioned minerals are in the divalent form and, in the fetus, are transported via DMT1 [129,134,135,136]. ZnT1, zinc transporter 1; MT1A, metallothionine-1A; ZIP14, zinc-importing protein; DMT1, divalent metal transporter 1; CTR1, copper transporter protein 1; Cu-Zn SOD, copper zinc superoxide dismutase; ATOX1, antioxidant 1 copper chaperone; ATP7A, ATPase copper-transporting alpha; TfR1, transferrin 1 receptor.
Figure 5. Proposed mechanism of fetomaternal transport of Fe, Mn, Zn, and Cu in cattle. Iron or manganese can form complexes with transferrin and bind to TfR1 in the placenta, which transports Fe or Mn to the fetus [135,137]. Cu and Zn are also transported by placental transporters CTR1 or Cu-Zn SOD [77,81,138,139] and ZIP14 [75], respectively. All these mentioned minerals are in the divalent form and, in the fetus, are transported via DMT1 [129,134,135,136]. ZnT1, zinc transporter 1; MT1A, metallothionine-1A; ZIP14, zinc-importing protein; DMT1, divalent metal transporter 1; CTR1, copper transporter protein 1; Cu-Zn SOD, copper zinc superoxide dismutase; ATOX1, antioxidant 1 copper chaperone; ATP7A, ATPase copper-transporting alpha; TfR1, transferrin 1 receptor.
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Table
Table 1. Mineral requirements and maximum tolerable limits during pregnancy as established by the National Academies of Sciences, Engineering, and Medicine (NASEM) for cattle.
Table 1. Mineral requirements and maximum tolerable limits during pregnancy as established by the National Academies of Sciences, Engineering, and Medicine (NASEM) for cattle.
Mineral Requirements of Dairy Cattle aMineral Requirements of Beef Cattle bMaximum Tolerable Level (MTL) c
MineralLactating CowDry Pregnant CowGrowing HeiferGrowing and Finishing CowGestating CowEarly Lactating Cow
Calcium, % d0.590.350.450.60.250.31.5
Phosphorous, %0.360.20.210.220.170.210.7
Magnesium, %0.170.140.120.10.120.200.40
Potassium, %1.020.660.560.60.60.72
Sodium, %0.220.170.160.06–0.080.06–0.080.13
Sulfur, %0.20.20.20.150.150.150.4
Cobalt, mg/kg d0.20.20.20.150.150.1525
Copper, mg/kg918.515.7510101040
Iodine, mg/kg0.440.530.550.50.50.550
Iron, mg/kg17.61432.5505050500
Manganese, mg/kg2840.541.252040402000
Selenium, mg/kg0.30.30.30.10.10.15
Zinc, mg/kg60.83136.5303030500
a Nutrient Requirements of Dairy Cattle from the NASEM, 2021 [42]; b Nutrient Requirements of Beef Cattle by the NASEM, 2016 [43]; c Mineral maximum tolerable levels (MTL) established for cattle by the NASEM, 2005 [44]; d % of dry matter and mg/kg of dry matter.
Table
Table 2. Maternal mineral nutrition associated with epigenomic regulation of the developing fetus.
Table 2. Maternal mineral nutrition associated with epigenomic regulation of the developing fetus.
MineralModelEpigenome RegulationOrganEffectReference
CaRatHypomethylation of CpG dinucleotide in promotor of hydroxysteroid 11-beta dehydrogenase 1 (Hsd11b1)LiverInduction of insulin resistance in adult life[118]
MgRat (Mg deficient model)Hypermethylation of CpG dinucleotide in promotor of 11β-hydroxysteroid dehydrogenase-2 (Hsd11b2)LiverAlters neonatal hepatic glucocorticoid metabolism[119]
FeRat (Fe deficient model)Hypomethylation at CpG site and reduction in histone H4 acetylation in promoter of brain-derived neurotrophic factor (BDNF)Brain (hippocampus)Crucial for regulation of hippocampal plasticity and development of neural circuit[120]
FeRat (Fe deficient model)Hypermethylation in 63 genes and hypomethylation in 45 genesBrain (hippocampus)Neural function dysregulation and alterations in cell-to-cell signal transduction [121]
FeDomestic pig (Fe deficient model)Twelve differentially methylated cytosines regulating nine differentially expressed genes were identifiedBrain (hippocampus)Associated genes were found to be involved in angiogenesis and neurodevelopment[122]
ZnMouse (Zn deficient model)Elevated expression of metallothionine-2 (MT2) mRNA response to histone modifications in metal-responsive elements associated with the promotor region of MT2LiverEpigenetic memory of zinc deficiency in early development may persist to adulthood, impacting availability of essential trace minerals[123]
SeRainbow trout (Se deficient model)Selenium availability affected the differentially methylated cytosines of more than 6500 differentially methylated genesLiverThe 6500 differentially methylated genes were found to be associated with immune modulations and neural signaling[124]
CuHumansCopper levels positively coincided with DNA methylation at CpG island and transcription site of Zinc Finger Protein 197 (ZNF197)PlacentaCan alter placentation and growth in postnatal life by impairing growth hormone secretion[125]
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Anas, M.; Diniz, W.J.S.; Menezes, A.C.B.; Reynolds, L.P.; Caton, J.S.; Dahlen, C.R.; Ward, A.K. Maternal Mineral Nutrition Regulates Fetal Genomic Programming in Cattle: A Review. Metabolites 2023, 13, 593. https://doi.org/10.3390/metabo13050593

AMA Style

Anas M, Diniz WJS, Menezes ACB, Reynolds LP, Caton JS, Dahlen CR, Ward AK. Maternal Mineral Nutrition Regulates Fetal Genomic Programming in Cattle: A Review. Metabolites. 2023; 13(5):593. https://doi.org/10.3390/metabo13050593

Chicago/Turabian Style

Anas, Muhammad, Wellison J. S. Diniz, Ana Clara B. Menezes, Lawrence P. Reynolds, Joel S. Caton, Carl R. Dahlen, and Alison K. Ward. 2023. "Maternal Mineral Nutrition Regulates Fetal Genomic Programming in Cattle: A Review" Metabolites 13, no. 5: 593. https://doi.org/10.3390/metabo13050593

APA Style

Anas, M., Diniz, W. J. S., Menezes, A. C. B., Reynolds, L. P., Caton, J. S., Dahlen, C. R., & Ward, A. K. (2023). Maternal Mineral Nutrition Regulates Fetal Genomic Programming in Cattle: A Review. Metabolites, 13(5), 593. https://doi.org/10.3390/metabo13050593

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