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Review

How Does Protein Nutrition Affect the Epigenetic Changes in Pig? A Review

by
Pablo Jesús Marín-García
1 and
Lola Llobat
2,*
1
Departamento Producción y Sanidad Animal, Salud Pública y Ciencia y Tecnología de los Alimentos, Facultad de Veterinaria, Universidad Cardenal Herrera-CEU, CEU Universities, 46010 Valencia, Spain
2
Grupo de Fisiopatología de la Reproducción, Departamento Producción y Sanidad Animal, Salud Pública y Ciencia y Tecnología de los Alimentos, Facultad de Veterinaria, Universidad Cardenal Herrera-CEU, CEU Universities, 46010 Valencia, Spain
*
Author to whom correspondence should be addressed.
Animals 2021, 11(2), 544; https://doi.org/10.3390/ani11020544
Submission received: 31 January 2021 / Revised: 16 February 2021 / Accepted: 17 February 2021 / Published: 19 February 2021
(This article belongs to the Section Animal Nutrition)

Abstract

:

Simple Summary

Epigenetic mechanisms regulate gene expression and depend of nutrition. In farm animals, and concretely, in pigs, some papers on protein nutrition have been realized to improve several productive traits. Changes in protein diet influence on epigenetic mechanisms that could affect productive and reproductive traits in individuals and their offspring. The purpose of this review was to update the current knowledge about the effects of these nutritional changes on epigenetic mechanisms in pigs.

Abstract

Epigenetic changes regulate gene expression and depend of external factors, such as environment and nutrition. In pigs, several studies on protein nutrition have been performed to improve productive and reproductive traits. Indeed, these studies aimed not only to determine broad protein requirements but also pigs’ essential amino acids requirements. Moreover, recent studies tried to determine these nutritional requirements for each individual, which is known as protein precision nutrition. However, nutritional changes could affect different epigenetic mechanisms, modifying metabolic pathways both in a given individual and its offspring. Modifications in protein nutrition, such as change in the amino acid profile, increase or decrease in protein levels, or the addition of metabolites that condition protein requirements, could affect the regulation of some genes, such as myostatin, insulin growth factor, or genes controlling cholesterol and glucose metabolism pathways. This review summarizes the impact of most common protein nutritional strategies on epigenetic changes and describes their effects on regulation of gene expression in pigs. In a context where animal nutrition is shifting towards precision protein nutrition (PPN), further studies evaluating the effects of PPN on animal epigenetic are necessary.

1. Introduction

The first definition of epigenetics was done in 1940 by Waddington [1]. Currently, different epigenetic regulation processes are known. The main acquaintances are DNA methylation, histone modifications, regulation by non-coding RNAs, such as microRNAs (miRNAs), and mechanisms that control chromatin organization. These processes can regulate gene expression independently of DNA sequence [2]. The first documented epigenetic modification was DNA methylation, and it was discovered in 1975, related to X-chromosome inactivation [3]. Lately, histone modifications and the role of chromatic structure in the regulation of the genome were elucidated [4]. The latest epigenetic regulation process discovered has been the non-coding RNA [5]. The influence of the environment on epigenetic changes has been demonstrated in plants and animals. Nutritional factors, such as levels of protein, and methyl group donors (some essential amino acids and other metabolites related to them) could also influence these epigenetic regulation [6,7]. In farm animals, different nutritional strategies are being investigated specifically in protein and amino acids content, which are directly related to both productive traits, as reduction of boar taint in meat, and to improve the meat quality [8,9]. These changes could have an epigenetic effect on animals, and their offspring. In this review, we summarize different strategies in pig’s nutrition, and their possible consequences in epigenetic regulation.

2. Nutrition in Pigs

Protein nutrition is essential in pig production, and it is being widely studied. Protein and amino acids have several functions (structural, regulatory, transporter, defensive, enzymatic, or even contractile) for animals, and they direct almost all life processes. Proteins are macro-biomolecules consisting of one or more amino acids chains, and they are synthesized from them, which become available either from the end products of digestion [10]. There exist two types of amino acids: those that the animals can synthesize (non-essential) and those that cannot synthesize by themselves (essential), and whether an amino acid is essential or not always depend on the species. Concretely, essential amino acids in pigs are methionine, lysine, histidine, isoleucine, leucine, phenylalanine, threonine, tryptophan, and valine, and they are necessary to control and provide by the diet, either though raw materials, or in some cases synthetically, due to the high nutritional requirements in livestock species.
Although protein and amino acids are considered nutrients (those components capable of being utilized by animals), some authors considered as additives, i.e., substances which, when incorporated in feeding-stuffs, are likely to affect their characteristics or livestock production [11] when they are added in a synthetic way. In this review, we refer to the presence of the nutrient regardless of whether it has been supplied by raw materials or synthetically.

2.1. Quality and Quantity of Protein

For the correct evaluation of the epigenetic effects of some nutrients, it is necessary to know the quality and quantity of them, and their interaction. In general terms, animals can be fed following two strategies, ad libitum or restricted. Regarding ad libitum system, the factor that will most affect the total amount of nutrients ingested will be the capacity of feed intake. Feed intake has been extensively studied both in growing animals [12], as well as reproductive animals [13,14], and it depends on many factors, like sex, breed, physiological state, environmental conditions, and housing system, but above all, it is also dependent of the quality of the diet [15,16,17]. Nevertheless, life weight is the parameter that reflects feed intake. There are certain physiological states (mainly pregnancy), when the animals are subjected to a food restriction, and this has direct effects on the total ingestion of protein and amino acids.
Regardless the nutrient quality, from the total crude protein (CP) ingested only a part, that is digested by enzymatic action and converted to amino acids and peptides [10], is absorbed into the stomach and, mainly, the small intestine [18]. This proportion corresponds with ileal digestible CP. The rest (ileal indigestible CP) goes to the large intestine, where it could be used or modified by the microbiota action (fecal digestible CP), or eliminated in feces (fecal indigestible CP). Digestible amino acids requirements could be calculated by either considering (real) or not (apparent) the endogenous flow (only the digestible fraction is capable of creating these epigenetic effects). For this reason, the formulation according to the digestible requirements at the true ileal levels is recommended; this is close to the ideal protein concept that refers to a situation where all essential amino acids are collimating for performance, so that the amino acids supply exactly matches the amino acids requirement [19]. In summary, a correct adjustment will lead to a better productivity, less pollution, and better health, thus improving the welfare state of the animals.
For the aforementioned, a large number of works to find the ideal protein have been performed in some productive species [20,21,22], including pigs. Usually, amino acid requirements have been determined by using dose–response methods which show the response of the performance to ascending contents of the amino acid studies [23]. However, there exist other techniques, such as controlling the amount of amino acid (in blood, plasma or serum), or even plasmatic urea nitrogen, which corresponds to the amount of nitrogen in form or urea circulating in the bloodstream [24]; it could be related with performance in pigs [25,26]. Nitrogen from unused amino acids presents an energy cost for the animal—three ATP molecules for every nitrogen molecule excreted [27]—related to the urea cycle. For this reason, not taking advantage of protein has a negative impact on two major aspects, as more energy used and more protein excreted. Furthermore, certain nutrients affect the requirements of another. In fact, methionine supplies methyl groups, and they are used in several metabolic pathways. These methyl groups also can be donated by choline, but both are eventually converted to betaine throughout these metabolic pathways. For this reason, an increase in both (choline and betaine) could minimize the use of methionine by these metabolic pathways, and therefore, its nutritional requirements [28,29].

2.2. Ideal-Protein Concept

Formulation according ideal protein is possible only if accurate knowledge exists about the requirements for all amino acids [19]. Currently, the global requirements for animals are widely studied, and they are collected in Figure 1, where current recommendations of protein according different physiological phases of pig production are shown [30,31,32]. These values are well-established for the medium of animals, but obviously they are not good for all animals. To be able to formulate into ideal protein, it is necessary to know the optimal nutritional requirements for each animal type, and there are several aspects that affect nutritional requirements, such feed efficiency, breed, environment, and performance, among others [33]. For this reason, there are many trials that try to relate the essential amino acid profile in the optimization both productive and reproductive traits, and some are developed below. Some works have studied the effects of lysine [25,33,34], methionine [35], arginine, and other essential amino acids [35,36,37,38,39,40] in several productive traits, like life weight, feed intake, feed conversion ratio, retention, or digestion. These results are explained by the greater availability of both protein and energy that allows the animals to optimize their productive traits. The different levels of amino acids not only affect growing pigs; this profile affects reproductive traits in pregnancy and lactating sows, uterine regression, milk and colostrum production, placenta and membrane functions, fetus growing, total piglets born, and weaned pigs, among others. Some works have studied the effects of lysine [23,41,42,43], methionine [44,45], arginine, valine, threonine, and tryptophan [26,43,46] in all parameters described above.
Several studies have been carried out in order to determine the optimal levels of amino acids for each stage in the life of the animal, which is leading towards the concept of precision protein nutrition (PPN). This PPN would try to assess the needs of the main amino acids in real time [47]. Thus, this new approach to animal nutrition is completely dynamic and requires continuous changes in the diet, to adapt to each situation [36]. This solution could minimize the epigenetic effects of an excess or lack of protein (or a certain amino acids) in animals, and specifically in pigs.

3. Epigenetic Modifications

3.1. DNA Methylation

DNA methylation is an essential process to regulate some biological functions in mammals, such as chromosomal stability, genomic imprinting, and X-chromosome inactivation. It occurs when methyl groups are added to the cytosine of CpG islands (Figure 2) [48]. This addition is catalyzed of three conserved enzyme families in mammals, DNA methyltransferase 1 (DNMT1), DNMT3a, and DNMT3b, which are essential to mammalian development and biological functions [49,50,51]. While DNMT1 maintains the methylation patterns during DNA replication, DNMT3a and DNMT3b are de novo methyltransferases [52]. The DNMT1 protein is expressed in somatic tissues and proliferating cells, and several isoforms have been detected [53,54]. In the case of DNMT3a and DNMT3b, alternative transcripts have been detected in the human and mouse [55].
To realize their function, these enzymes need a methyl donor, so they are directly influenced by methyl groups derived from the diet, such as choline/betaine, methyl-folate, or methionine, that are precursors to the universal methyl-donor S-adenosylmethionine (SAM) [56,57,58,59]. An example is the regulation of insulin-like growth factor II (IGF2), which is negatively regulated by a H19 gene, that regulation, in turn, depends of concrete region methylation, Igf2DMR2. Pregnant rats with a choline-deficient diet presented hypermethylation of these regions, so H19 is inhibited and IGF2 expression increases [60]. Epigenetic regulation of this gene and its relationship with nutrition have been well-known since the Dutch Hunger Winter in 1944/1945 in humans, when pregnant women exposed to famine had descendants with less DNA methylation at the IGF2 gene, and these losses were maintained up to 60 years [61]. In livestock, different authors indicate the relevance of nutrition in epigenetic marks. Murdoch et al. (2016) published an extensive review about the methylation effect of quality and quantity of nutrients in different livestock species [62]. The most important nutrient related to epigenetic effects and, concretely, with effect in DNA methylation, are methyl group donors, such as methionine or another methyl group donor used as an alternative to methionine (mainly, folate and betaine). Betaine injections in eggs increase DNA methylation, regulating hepatic cholesterol metabolism in chicks [63]. Moreover, pregnant sows that were fed with betaine-supplemented diets presented modifications of methylation patterns in newborn piglets [64]. In sheep, deficient diets in vitamin B12, folate, and methionine provoke hypomethylation in offspring that relates to birth weight, alterations in immune responses, and elevation of blood pressure [61].
Quantitative trait loci (QTL) have been found in pig for most economically important traits, such as carcass and meat quality [65,66,67]. Some of these QTL are regulated by methylation [68,69] or another epigenetic mechanism [70] and could affect phenotypic variation in livestock production. Therefore, studies on epigenetic regulation, and specifically through DNA methylation of characters of interest for livestock production, would be necessary, mainly from the point of view of how the nutrition of animals affects these methylation changes.

3.2. Histone Modifications

Since 1964, the post-translational modifications of histones have been well-known [71]. Acetylation, phosphorylation, and methylation of histones could affect chromatin structure and influence transcription and gene expression (Figure 3) [72]. Modifications in histone 1 (H1) (linker histone), H2A, H2B, H3, and H4 core histone families are related to different functions, such as chromatin dynamics, transcriptional activation, heterochromatin formation, telomere stabilization, or gene silencing, among others. These functions could regulate gene expression and develop as different genetic disorders or early development in mammals [73,74,75].
Acetylation occurs in lysine residues of histones, and it regulates by two families of enzymes, histone acetyltransferases (HATs) and histone deacetylases (SDCAs). The HATs catalyze the transfer of an acetyl group of lysine side chain, whereas HDAC enzymes catalyze the reverse process [76]. Histone phosphorylation takes place on serine, threonine, and tyrosine and is regulated by kinases and phosphatases [77]. Finally, histone methylation is carried out on the side chain of lysine and arginine, with specific methylases and demethylases [78,79]. Histone modifications are related to the regulation of multiple biological process. One of the most important process regulated by histone modifications is the early mammalian development. One example is the formation of the trophectoderm and the inner cell mass that is related to modifications in histone 3, concretely in the 4 and 27 lysine residues (H3K4 and H3K27) in mouse embryos [80]. Histone modifications are necessary for more complex regulatory mechanisms in vivo. Indeed, histone methylation is related to genomic imprinting, HOX gene expression, and the regulation of pluripotency in mammalian early development [81].
Some studies indicate the relationship between different nutrients and histone modifications. Regarding that, one of the most studied nutrients are vitamins. The availability of retinoic acid (RA), a natural derivative of vitamin A, modifies the histone patterns. RA treatment increases H3K4 and decreases H3K27, and it increases H3K9 and H3K14 acetylation in humans [82]. A diet deficient of vitamin A decreases HAT activity and H3 and H4 histones acetylation in rats [83]. Another vitamin that affects histone modifications is vitamin C, which is also linked with the reduction of H9K9 dimethylation in mouse embryonic stem cells [84]. Other compounds of diets related to histone modifications are organosulfur compounds, sodium butyrate, genistein, bioflavonoids, or catechins [85]. Studies related to effect of vitamins or other nutrients in farm animals are not carried out, except related to protein levels. Deficient-protein diets improve H3 acetylation in the promotor of myostatin gene that produces alterations in gene expression in pigs [86,87].

3.3. Small Non-Coding RNA: miRNAs as Epigenetic Regulators

In 1993, the first miRNA lin-4 was discovered in the nematode Caenorhabditis elegans, but its importance was only understood after the discovery of a second miRNA, let-7 [88,89]. MiRNAs are small non-coding RNA molecules of approximately 20–24 pairs in length, are therefore they are unable to code for proteins [90,91,92]. They are usually phylogenetically conserved and have been shown to play a crucial role in the regulation of gene expression and cellular processes [92,93]. Since their discovery, thousands of miRNAs have been identified, and their presence or absence regulates different functions in different organisms. The biogenesis of miRNAs is a complex process that requires two endonucleases, Drosha and Dices, and the nuclear transport receptor Exportin 5 (XPO5) (Figure 4) [94]. The miRNAs, along with other less-known non-coding RNAs, as piwi-interacting RNA (piRNA), small-interfering RNA (siRNA), and small nucleolar RNA (snoRNA), regulate gene expression in some mechanism, including heterochromatin formation and inhibition of translation [95,96,97].
Like other epigenetic regulators, miRNAs could also be affected by nutrients. Expression of miRNAs could also be influenced by vitamins, so RA regulates the miRNAs expression in different biological tissues, such as embryos, the heart, muscles, or nervous tissue [99]. Moreover, low-protein diets provoke the reduction of miR-136 and miR-500, affecting myostatin gene expression in pigs [87].

3.4. Other Non-Coding RNAs as Epigenetic Regulators

Additionally, other non-coding RNAs appear to act as epigenetic regulators. For instance, there is a growing body of evidence suggesting that small interfering RNAs (siRNAs), small nucleolar RNAs (snoRNAs), circular RNAs (circRNAs), piwi-interacting RNAs (piRNAs), or long non-coding (lncRNAs) have a pivotal role in the epigenetic landscape (reviewed elsewhere [100,101,102]). However, the direct relationship between these non-coding RNAs and nutrition still remains unknown. Table 1 summarizes different non-coding RNAs and their impact in epigenetics.

4. Epigenetic Effect of Diets in Pigs

4.1. Effect of Protein Levels

Different studies have shown the effects of high or low amounts of protein in the diet, on the regulation of gene expression. The first trials indicated an increase in the mRNA expression of renal renin when rats were fed a high-protein diet, which can lead to kidney diseases [113,114]. A similar effect has been detected in liver, where an increase of protein in the diet provokes cellular retinol binding protein I (CRPB I) overexpression [115]. However, not only the protein quantity affects the regulation of genes, but the quality of this protein also alters expression profiles. Endo et al. (2002) observed different expression of 111 genes in rats fed with casein than rats fed with wheat gluten, and drastic changes in expression of DNA-binding inhibitor protein (involved in the regulation of multiple genes) were detected [116]. These results could have a relationship with the different digestibility of these two protein sources [117]. On the other hand, high protein levels increase the gene expression of enzyme serine dehydratase in the liver, related to gluconeogenesis, and causing weight gain in these animals probably [118]. Other studies have analyzed the effect of different amounts of protein in the diet of pregnant females. The results indicated that low protein levels increase the expression of genes related to p53 pathways and negative regulators of cell growth and metabolism, in addition to genes involved in epigenetic changes [119]. These changes in DNA methylation due to a low protein diet seem to be able to be alleviated with a supplementation in methyl group donors, such as folate [120].
The effect of changes of protein diet have also been seen in pigs. For example, in sows, low levels of protein resulted in an increase in myostatin gene expression at weaning; however, the authors did not find differential expression of the 12 miRNAs analyzed, related to the regulation of the expression of this gene [87]. A decrease in the expression of miRNAs as ssc-miR-136 and ssc-miR-500 has been demonstrated, but the regulatory path is not clear yet [87]. Evidence that the level of protein in the diet affects epigenetic regulation has been demonstrated in different studies in pigs. Altmann et al. (2012) observed a different expression of demethylation enzymes DNMT1, DNMT3a, and DNMT3b, with high and low protein diets during porcine pregnancy in skeletal muscle and liver expression patterns [121]. In a posterior study, same authors detected different methylation patterns in metabolic genes with high and lower levels of protein in the diet of pregnancy sows [122], which shows that the amount of protein ingested by the mother during pregnancy has a direct effect on methylation patterns and, therefore, on the epigenetic regulation of the offspring. In accordance with that, low levels of protein in pregnant sows give rise to hypomethylation of the promotor of 3-hydroxy-3-methylgluratyl-CoA reductase (HMGCR) gene (related to cholesterol biosynthesis), and with the decrease of H3 histone monomethylation, lysine 9 of H3 histone monomethylation, and lysine 27 of H3 histone trimethylation, as well as the increase of H3 acetylation, among other epigenetic changes [123]. Besides these effects on cholesterol metabolism and its epigenetic regulation, low protein levels influence the regulation of the insulin growth factor system, decreasing IGF-I levels in liver by the regulation of rapamycin (mTOR) and peroxisome proliferator–activated receptor γ (PPAR γ) interaction [124]. Thus, pregnant sows fed with low- and high-protein diets during pregnancy presented changes in protein and fats metabolism, causing a delay in fetal growth and low birth weights of the offspring [125]. Low levels of protein affect the formation of prenatal myofibers, and they reduce the expression of IGF2 and change the quality of the carcass [126]. These results indicate that a protein imbalance during pregnancy alters the regulation of these metabolic pathways in sows and their offspring, and a deficiency in protein in the maternal diet alters meat quality. Some authors attribute these changes to the imbalance of some micronutrients, as certain essential amino acids, or molecules, such as methyl group donors. For this reason, in the following sections of this review, these metabolites are analyzed individually.

4.2. Effect of Methyl Group Donors

Some amino acids, mainly methionine, participate in the in one-carbon-unit metabolism that regulates the synthesis of purines and methylation. Other metabolites, such as betaine, choline, and folate, are used to provide methyl donor for methyltransferases, and their use is related with amino acids requirements. All of them have an important role in the regulation of SAM (Figure 5) [127].
Regarding these methyl group donors, one of the most studied in pregnant sows has been betaine. Betaine is a substrate for the formation of methionine, and further studies indicate that betaine supplementation may modulate gene expression by DNA and histone methylation in human [128,129]. In pigs, the Zhao research group has carried out several studies, in which the epigenetic influence of betaine supplementation in the diet of pregnant sows has been demonstrated. Concretely, this supplementation increases liver cholesterol, changes the expression of different genes related to gluconeogenesis metabolism, and inhibits liver cells proliferation. For example, IGF2 gene affects gluconeogenesis, and its expression in the hippocampus of newborn piglets is controlled by different epigenetic mechanisms, such as DNA methylation, histone modifications, and expression or repression of some miRNAs [64,130,131,132]. The effects of a deficiency in folate and their relationship between epigenetic regulation have been extensively studied in humans [133]. In pigs, studies are not as extensive; however, a similar effect of betaine on DNA methylation in piglets has been demonstrated [134]. Recently, He et al. (2020) studied the effect of methyl donors, such as folate, choline, and methionine supplementation in pregnant sows, and the results showed an increase of proteins of one-carbon-unit metabolism in females and piglets, and skeletal muscle differentiation increase in piglets, probably regulated by epigenetic modifications [135]. However, since, in this study, the supplementation was performed with all the methyl group donors simultaneously, the effect of each of them in pigs remains to be discovered.
Some studies have been realized in other mammalian species and demonstrated the beneficial effect of methionine supplementation in epigenetic mechanisms. On one hand, methionine supplementation in rats is capable of inhibiting the expression of DNMT1 and histone methylation, thereby preventing epigenetic alterations induced by diabetes [136]. On the other hand, the methionine supplementation in the diet of pregnant female cattle increases DNMT3a, whereas global DNA methylation is lower in placenta [137]. Considering that the methylation state fluctuates throughout the sow’s reproductive cycle [138], studies that analyze the effect of methionine supplementation in this species are necessary, and they could have more relationship about an imbalance in the quality of the protein (essential amino acid profile).

4.3. Effect of Lysine

Lysine is one of the essential amino acids in pigs, and the requirements are higher than other essential amino acids. Regarding epigenetic mechanisms, both histone acetylation and histone methylation occurs in lysine residues of histones [76,79]. Methylation of lysine residues of non-histones protein has been discovered with another mechanism of post-translational regulation that regulates chromatin remodeling, gene transcription, protein synthesis, signal transduction, and DNA repair [139].
Lysine deficiency in pigs affects different productive traits. Low levels of lysine in pig diets decrease the average daily gain and loin percentage, and increase feed-to-gain conversion ratio, back-fat thickness, and intramuscular fat content [140,141]. The molecular mechanisms that produce these effects are unknown; however, some studies have shown that diets with a low lysine content decrease the expression of some genes, such as genes that code for amino acid transporters and muscle growth, such as myosin [142,143]. Low levels of lysine cause a reduction in IGF-1 plasmatic levels, without decreasing the levels of its mRNA in the liver, suggesting a post-transcriptional regulation [144]. Although these findings seem to point to an influence of lysine deficiency on gene regulation, either pre- or post-translational, more studies will be necessary to find out the regulatory processes that underlie these changes in production parameters.
About the effects of lysine excess, most authors agree on the low toxicity of lysine, mainly due to a slow entry of it into the bloodstream, good elimination through urine, longer time for release of lysine from circulation to muscle during storage, and liver metabolism [145]. Nonetheless, hyperlysinemia has been related to mental motor retardation, seizures, muscle hypotonia, spasticity, abdominal cramps, and diarrhea in humans [146,147]. Studies in pigs, in this regard, are scarce. For example, Edmonds and Baker (1987) founded a decrease of daily weight and food intake when animals were fed with higher lysine levels [148]. As with lysine deficiency, the underlying mechanisms are unknown.
Continuing to research the effects of the excess and deficiency of lysine both in production parameters and in mechanisms of epigenetics regulation would be of high interest for the swine industry and for animal nutrition.

5. Conclusions

This review analyzed different effects of both protein and amino acid levels in the diet, on different epigenetic regulatory mechanisms, such as DNA methylation, histone modifications, and regulation by non-coding RNAs (miRNA). Given that nutritional requirements are variable for each animal and changing in a dynamic way, new animal nutrition techniques go towards precision protein nutrition. In this context, where amino acid content is variable, it is important to know the effects of how these different levels of proteins and amino acids could modify these epigenetic changes, since these interactions not only affect the productive traits of the animal, but also other traits both of its own and of its offspring.

Author Contributions

Writing—original draft preparation, P.J.M.-G. and L.L.; writing—review and editing, P.J.M.-G. and L.L.; supervision, L.L. All authors have read and agreed to the published version of the manuscript.

Funding

This research received no external funding.

Institutional Review Board Statement

Not applicable.

Data Availability Statement

Not applicable.

Acknowledgments

We are grateful to Veterinary Medicine Faculty to Universidad Cardenal Herrera, CEU.

Conflicts of Interest

The authors declare no conflict of interest.

Abbreviations

CPtotal crude protein
CRBPcellular retinol binding protein
DNMTDNA methyltransferase
HHistone
HAThistone acetyltransferase
HDAChistone deacetylase
HMGCR3-hydroxy-3-methylglutary-CoA reductase
IGFInsulin growth factor
miRNAmicroRNA
mTORrapamycin
piRNApiwi-interacting RNA
PPARγperoxisome proliferator-activated receptor γ
PPNprecision protein nutrition
QTLquantitative trait loci
RAretinoic acid
RISCRNA induced silencing complex
SAMS-adenosylmethionine
siRNAsmall-interfering RNA
snoRNAsmall nucleolar RNA
XPO5exportin 5

References

  1. Haldane, J.B.S. Organisers and Genes. Nature 1940, 146, 413. [Google Scholar] [CrossRef]
  2. Jirtle, R.L.; Skinner, M.K. Environmental epigenomics and disease susceptibility. Nat. Rev. Genet. 2007, 8, 253–262. [Google Scholar] [CrossRef] [PubMed]
  3. Holliday, R.; Pugh, J. DNA modification mechanisms and gene activity during development. Science 1975, 187, 226–232. [Google Scholar] [CrossRef] [PubMed]
  4. Turner, B.M. Histone acetylation as an epigenetic determinant of long-term transcriptional competence. Cell. Mol. Life Sci. 1998, 54, 21–31. [Google Scholar] [CrossRef]
  5. Pokholok, D.K.; Harbison, C.T.; Levine, S.; Cole, M.; Hannett, N.M.; Lee, T.I.; Bell, G.W.; Walker, K.; Rolfe, P.A.; Herbolsheimer, E.; et al. Genome-wide Map of Nucleosome Acetylation and Methylation in Yeast. Cell 2005, 122, 517–527. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  6. Cooney, C.A.; Dave, A.A.; Wolff, G.L. Maternal Methyl Supplements in Mice Affect Epigenetic Variation and DNA Methylation of Offspring. J. Nutr. 2002, 132, 2393S–2400S. [Google Scholar] [CrossRef] [Green Version]
  7. Cropley, J.E.; Suter, C.M.; Beckman, K.B.; Martin, D.I.K. From the Cover: Germ-line epigenetic modification of the murine Avy allele by nutritional supplementation. Proc. Natl. Acad. Sci. USA 2006, 103, 17308–17312. [Google Scholar] [CrossRef] [Green Version]
  8. Bee, G.; Quiniou, N.; Maribo, H.; Zamaratskaia, G.; Lawlor, P.G. Strategies to Meet Nutritional Requirements and Reduce Boar Taint in Meat from Entire Male Pigs and Immunocastrates. Animals 2020, 10, 1950. [Google Scholar] [CrossRef]
  9. Ma, X.; Yu, M.; Liu, Z.; Deng, D.; Cui, Y.; Tian, Z.; Wang, G. Effect of amino acids and their derivatives on meat quality of finishing pigs. J. Food Sci. Technol. 2020, 57, 404–412. [Google Scholar] [CrossRef]
  10. Animal Nutrition—Peter McDonald—9781408204238—Agriculture—Animal Science (80). Available online: https://www.pearson.ch/HigherEducation/Pearson/EAN/9781408204238/Animal-Nutrition (accessed on 21 January 2021).
  11. Council Directive 70/524/EEC of 23 November 1970 Concerning Additives in Feeding-Stuffs; The Council of the European Communities: Bruxelles, Belgium, 1970; Available online: https://eur-lex.europa.eu.
  12. Knap, P.W. Variation in Maintenance Requirements of Growing Pigs in Relation to Body Composition: A Simulation Study. Ph.D. Thesis, Wageningen University, Wageningen, The Netherlands, 2000. [Google Scholar]
  13. National Research Council. Predicting Feed Intake of Food-Producing Animals; The National Academies Press: Washington, DC, USA, 1987; ISBN 9780309036955. [Google Scholar]
  14. National Research Council. Nutrient Requirements of Swine: 10th Revised Edition; The National Academies Press: Washington, DC, USA, 1999. [Google Scholar]
  15. Quiniou, N.; Dubois, S.; Noblet, J. Voluntary feed intake and feeding behaviour of group-housed growing pigs are affected by ambient temperature and body weight. Livest. Prod. Sci. 2000, 63, 245–253. [Google Scholar] [CrossRef]
  16. Rayner, D.V.; Gregory, P.C. The rôle of the gastrointestinal tract in the control of voluntary food intake. BSAP Occas. Publ. 1989, 13, 27–39. [Google Scholar] [CrossRef]
  17. Whittemore, C.; Kerr, J.; Cameron, N. An approach to prediction of feed intake in growing pigs using simple body measurements. Agric. Syst. 1995, 47, 235–244. [Google Scholar] [CrossRef]
  18. D’Mello, J.P.F. Amino Acids in Animal Nutrition, 2nd ed.; CABI: Wallingford, UK, 2003; ISBN 9780851996547. [Google Scholar]
  19. Van Milgen, J.; Dourmad, J.-Y. Concept and application of ideal protein for pigs. J. Anim. Sci. Biotechnol. 2015, 6, 15. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  20. Belloir, P.; Méda, B.; Lambert, W.; Corrent, E.; Juin, H.; Lessire, M.; Tesseraud, S. Reducing the CP content in broiler feeds: Impact on animal performance, meat quality and nitrogen utilization. Animal 2017, 11, 1881–1889. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  21. Dairo, F.A.S.; Fajemilehin, S.O.K.; Adegun, M.K.; Adelabu, D.B.; Balogun, A.K. Carcass, Organs and Economic Evaluation of Broiler Birds Fed Low-protein Diets Supplemented with the Most Limiting Essential Amino Acids in Ideal Protein Concept. J. Exp. Agric. Int. 2017, 18, 1–10. [Google Scholar] [CrossRef]
  22. Marín-García, P.J.; López-Luján, M.C.; Ródenas, L.; Martínez-Paredes, E.M.; Blas, E.; Pascual, J.J. Plasmatic Urea Nitrogen in Growing Rabbits with Different Combinations of Dietary Levels of Lysine, Sulphur Amino Acids and Threonine. Animals 2020, 10, 946. [Google Scholar] [CrossRef] [PubMed]
  23. Coma, J.; Zimmerman, D.R.; Carrion, D. Lysine requirement of the lactating sow determined by using plasma urea nitrogen as a rapid response criterion. J. Anim. Sci. 1996, 74, 1056–1062. [Google Scholar] [CrossRef] [Green Version]
  24. Marín García, P.J.; del López Luján, M.C.; Ródenas Martínez, L.; Martínez-Paredes, E.M.; Blas Ferrer, E.; Pascual Amorós, J.J. Plasma Urea Nitrogen as an Indicator of Amino Acid Imbalance in Rabbit Diets. In Proceedings of the World Rabbit Science; Universitat Politècnica de València: Valencia, Spain, 30 June 2020; Volume 28, pp. 63–72. [Google Scholar]
  25. Nieto, R.; Barea, R.; Lara, L.; Palma-Granados, P.; Aguilera, J. Lysine requirement relative to total dietary protein for optimum performance and carcass protein deposition of Iberian piglets. Anim. Feed Sci. Technol. 2015, 206, 48–56. [Google Scholar] [CrossRef]
  26. Roth-Maier, D.A.; Ott, H.; Roth, F.X.; Paulicks, B.R. Effects of the level of dietary valine supply on amino acids and urea concentration in milk and blood plasma of lactating sows. J. Anim. Physiol. Anim. Nutr. 2004, 88, 39–45. [Google Scholar] [CrossRef]
  27. Bohinski, R.C. Modern Concepts in Biochemistry, 2nd ed.; Allyn & Bacon: Boston, MA, USA, 1987. [Google Scholar] [CrossRef]
  28. Eklund, M.; Bauer, E.; Wamatu, J.; Mosenthin, R. Potential nutritional and physiological functions of betaine in livestock. Nutr. Res. Rev. 2005, 18, 31–48. [Google Scholar] [CrossRef] [Green Version]
  29. Matthews, J.O.; Southern, L.L.; Pontif, J.E.; Higbie, A.D.; Bidner, T.D. Interactive effects of betaine, crude protein, and net energy in finishing pigs. J. Anim. Sci. 1998, 76, 2444–2455. [Google Scholar] [CrossRef] [PubMed]
  30. Chastanet, F.; Pahm, A.; Pedersen, C.; Stein, H. Effect of feeding schedule on apparent energy and amino acid digestibility by growing pigs. Anim. Feed Sci. Technol. 2007, 132, 94–102. [Google Scholar] [CrossRef]
  31. Fuller, M.F.; McWilliam, R.; Wang, T.C.; Giles, L.R. The optimum dietary amino acid pattern for growing pigs. 2. Requirements for Maintenance and for Tissue Protein Accretion. Br. J. Nutr. 1989, 62, 255–267. [Google Scholar] [CrossRef] [PubMed]
  32. Nieto, R.; Rivera, M.; García, M.; Aguilera, J. Amino acid availability and energy value of acorn in the Iberian pig. Livest. Prod. Sci. 2002, 77, 227–239. [Google Scholar] [CrossRef]
  33. Brossard, L.; Dourmad, J.-Y.; Rivest, J.; Van Milgen, J. Modelling the variation in performance of a population of growing pig as affected by lysine supply and feeding strategy. Animal 2009, 3, 1114–1123. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  34. Andretta, I.; Pomar, C.; Rivest, J.; Pomar, J.; Radünz, J. Precision feeding can significantly reduce lysine intake and nitrogen excretion without compromising the performance of growing pigs. Animal 2016, 10, 1137–1147. [Google Scholar] [CrossRef] [Green Version]
  35. Remus, A.; Pomar, C.; Perondi, D.; Gobi, J.; Da Silva, W.; De Souza, L.; Hauschild, L. Response to dietary methionine supply of growing pigs fed daily tailored diets or fed according to a conventional phase feeding system. Livest. Sci. 2019, 222, 7–13. [Google Scholar] [CrossRef]
  36. Hauschild, L.; Lovatto, P.A.; Pomar, J.; Pomar, C. Development of sustainable precision farming systems for swine: Estimating real-time individual amino acid requirements in growing-finishing pigs. J. Anim. Sci. 2012, 90, 2255–2263. [Google Scholar] [CrossRef]
  37. Kerr, B.J.; Yen, J.T.; Nienaber, J.A.; Easter, R.A. Influences of dietary protein level, amino acid supplementation and environmental temperature on performance, body composition, organ weights and total heat production of growing pigs. J. Anim. Sci. 2003, 81, 1998–2007. [Google Scholar] [CrossRef] [Green Version]
  38. Lenehan, N.A.; Usry, J.L.; Hastad, C.W.; Barker, M.R.; Frantz, N.Z.; Groesbeck, C.N.; James, B.W.; Keegan, T.P.; Lawrence, K.R.; Young, M.G.; et al. The optimal true ileal digestible lysine and threonine requirement for nursery pigs between 25 and 55 lb. Kans. Agric. Exp. Stn. Res. Rep. 2003, 61–66. [Google Scholar] [CrossRef] [Green Version]
  39. Toledo, J.; Furlan, A.; Pozza, P.; Piano, L.; Carvalho, P.; Peñuela-Sierra, L.; Huepa, L. Effect of the reduction of the crude protein content of diets supplemented with essential amino acids on the performance of piglets weighing 6–15 kg. Livest. Sci. 2014, 168, 94–101. [Google Scholar] [CrossRef]
  40. Waguespack, A.M.; Bidner, T.D.; Payne, R.L.; Southern, L.L. Valine and isoleucine requirement of 20- to 45-kilogram pigs. J. Anim. Sci. 2012, 90, 2276–2284. [Google Scholar] [CrossRef] [PubMed]
  41. Dourmad, J.Y.; Noblet, J.; Étienne, M. Effect of protein and lysine supply on performance, nitrogen balance, and body composition changes of sows during lactation. J. Anim. Sci. 1998, 76, 542–550. [Google Scholar] [CrossRef]
  42. Feyera, T.; Theil, P.K. Energy and lysine requirements and balances of sows during transition and lactation: A factorial approach. Livest. Sci. 2017, 201, 50–57. [Google Scholar] [CrossRef]
  43. Soltwedel, K.T.; Easter, R.A.; Pettigrew, J.E. Evaluation of the order of limitation of lysine, threonine, and valine, as determined by plasma urea nitrogen, in corn-soybean meal diets of lactating sows with high body weight loss. J. Anim. Sci. 2006, 84, 1734–1741. [Google Scholar] [CrossRef] [PubMed]
  44. Azad, A.K.; Bin, P.; Liu, G.; Fang, J.; Li, T.; Yin, Y. Effects of different methionine levels on offspring piglets during late gestation and lactation. Food Funct. 2018, 9, 5843–5854. [Google Scholar] [CrossRef]
  45. Schneider, J.D.; Nelssen, J.L.; Tokach, M.D.; Goodband, R.D.; DeRouchey, J.M.; Dritz, S.S. Determining the total sulfur amino acid to lysine requirement of the lactating sow. Kans. Agric. Exp. Stn. Res. Rep. 2006, 47–51. [Google Scholar] [CrossRef] [Green Version]
  46. Figueroa, J.L.; Lewis, A.J.; Miller, P.S.; Fischer, R.L.; Gómez, R.S.; Diedrichsen, R.M. Nitrogen metabolism and growth performance of gilts fed standard corn-soybean meal diets or low-crude protein, amino acid-supplemented diets. J. Anim. Sci. 2002, 80, 2911–2919. [Google Scholar] [CrossRef] [PubMed]
  47. Cloutier, L.; Pomar, C.; Montminy, M.L.; Bernier, J.; Pomar, J. Evaluation of a method estimating real-time individual lysine requirements in two lines of growing–finishing pigs. Animal 2015, 9, 561–568. [Google Scholar] [CrossRef]
  48. Smith, Z.D.; Meissner, A. DNA methylation: Roles in mammalian development. Nat. Rev. Genet. 2013, 14, 204–220. [Google Scholar] [CrossRef]
  49. Hoang, N.-M.; Rui, L. DNA methyltransferases in hematological malignancies. J. Genet. Genom. 2020, 47, 361–372. [Google Scholar] [CrossRef] [PubMed]
  50. Okano, M.; Bell, D.W.; Haber, D.A.; Li, E. DNA Methyltransferases Dnmt3a and Dnmt3b Are Essential for De Novo Methylation and Mammalian Development. Cell 1999, 99, 247–257. [Google Scholar] [CrossRef] [Green Version]
  51. Zhang, J.; Yang, C.; Wu, C.; Cui, W.; Wang, L. DNA Methyltransferases in Cancer: Biology, Paradox, Aberrations, and Targeted Therapy. Cancers 2020, 12, 2123. [Google Scholar] [CrossRef]
  52. Hamidi, T.; Singh, A.K.; Chen, T. Genetic alterations of DNA methylation machinery in human diseases. Epigenomics 2015, 7, 247–265. [Google Scholar] [CrossRef] [PubMed]
  53. Deng, J.; Szyf, M. Multiple Isoforms of DNA Methyltransferase Are Encoded by the Vertebrate Cytosine DNA Methyltransferase Gene. J. Biol. Chem. 1998, 273, 22869–22872. [Google Scholar] [CrossRef] [Green Version]
  54. Leonhardt, H.; Bestor, T.H. Structure, function and regulation of mammalian DNA methyltransferase. DNA Methylation 1993, 64, 109–119. [Google Scholar] [CrossRef] [Green Version]
  55. Robertson, K.D.; Uzvolgyi, E.; Liang, G.; Talmadge, C.; Sumegi, J.; Gonzales, F.A.; Jones, P.A. The human DNA methyltransferases (DNMTs) 1, 3a and 3b: Coordinate mRNA expression in normal tissues and overexpression in tumors. Nucleic Acids Res. 1999, 27, 2291–2298. [Google Scholar] [CrossRef] [Green Version]
  56. Kok, D.E.G.; Dhonukshe-Rutten, R.A.M.; Lute, C.; Heil, S.G.; Uitterlinden, A.G.; Van Der Velde, N.; Van Meurs, J.B.J.; Van Schoor, N.M.; Hooiveld, G.J.E.J.; De Groot, L.C.P.G.M.; et al. The effects of long-term daily folic acid and vitamin B12 supplementation on genome-wide DNA methylation in elderly subjects. Clin. Epigenet. 2015, 7, 1–14. [Google Scholar] [CrossRef] [Green Version]
  57. Nilsson, E.A.; Matte, A.; Perfilyev, A.; De Mello, V.D.; Käkelä, P.; Pihlajamäki, J.; Ling, C. Epigenetic Alterations in Human Liver from Subjects with Type 2 Diabetes in Parallel with Reduced Folate Levels. J. Clin. Endocrinol. Metab. 2015, 100, e1491–e1501. [Google Scholar] [CrossRef]
  58. Salbaum, J.M.; Kappen, C. Genetic and Epigenomic Footprints of Folate. Prog. Mol. Biol. Transl. Sci. 2012, 108, 129–158. [Google Scholar] [CrossRef] [Green Version]
  59. Zeisel, S.H. Choline, Other Methyl-Donors and Epigenetics. Nutrients 2017, 9, 445. [Google Scholar] [CrossRef] [PubMed]
  60. Kovacheva, V.P.; Mellott, T.J.; Davison, J.M.; Wagner, N.; Lopez-Coviella, I.; Schnitzler, A.C.; Blusztajn, J.K. Gestational Choline Deficiency Causes Global and Igf2 Gene DNA Hypermethylation by Up-regulation of Dnmt1 Expression. J. Biol. Chem. 2007, 282, 31777–31788. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  61. Heijmans, B.T.; Tobi, E.W.; Stein, A.D.; Putter, H.; Blauw, G.J.; Susser, E.S.; Slagboom, P.E.; Lumey, L.H. Persistent epigenetic differences associated with prenatal exposure to famine in humans. Proc. Natl. Acad. Sci. USA 2008, 105, 17046–17049. [Google Scholar] [CrossRef] [Green Version]
  62. Murdoch, B.M.; Murdoch, G.K.; Greenwood, S.; McKay, S. Nutritional Influence on Epigenetic Marks and Effect on Livestock Production. Front. Genet. 2016, 7, 182. [Google Scholar] [CrossRef] [Green Version]
  63. Hu, Y.; Sun, Q.; Li, X.; Wang, M.; Cai, D.; Li, X.; Zhao, R. In Ovo Injection of Betaine Affects Hepatic Cholesterol Metabolism through Epigenetic Gene Regulation in Newly Hatched Chicks. PLoS ONE 2015, 10, e0122643. [Google Scholar] [CrossRef] [Green Version]
  64. Cai, D.; Jia, Y.; Song, H.; Sui, S.; Lu, J.; Jiang, Z.; Zhao, R. Betaine Supplementation in Maternal Diet Modulates the Epigenetic Regulation of Hepatic Gluconeogenic Genes in Neonatal Piglets. PLoS ONE 2014, 9, e105504. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  65. Liu, Y.; Liu, X.; Zheng, Z.; Ma, T.; Liu, Y.; Long, H.; Cheng, H.; Fang, M.; Gong, J.; Li, X.; et al. Genome-wide analysis of expression QTL (eQTL) and allele-specific expression (ASE) in pig muscle identifies candidate genes for meat quality traits. Genet. Sel. Evol. 2020, 52, 1–11. [Google Scholar] [CrossRef] [PubMed]
  66. Fabbri, M.C.; Zappaterra, M.; Davoli, R.; Zambonelli, P. Genome-wide association study identifies markers associated with carcass and meat quality traits in Italian Large White pigs. Anim. Genet. 2020, 51, 950–952. [Google Scholar] [CrossRef] [PubMed]
  67. Hu, Z.-L.; Dracheva, S.; Jang, W.; Maglott, D.; Bastiaansen, J.; Rothschild, M.F.; Reecy, J.M. A QTL resource and comparison tool for pigs: PigQTLDB. Mamm. Genome 2005, 16, 792–800. [Google Scholar] [CrossRef] [Green Version]
  68. Fan, Y.; Vilgalys, T.P.; Sun, S.; Peng, Q.; Tung, J.; Zhou, X. IMAGE: High-powered detection of genetic effects on DNA methylation using integrated methylation QTL mapping and allele-specific analysis. Genome Biol. 2019, 20, 1–18. [Google Scholar] [CrossRef] [Green Version]
  69. Gibbs, J.R.; Van Der Brug, M.P.; Hernandez, D.G.; Traynor, B.J.; Nalls, M.A.; Lai, S.-L.; Arepalli, S.; Dillman, A.; Rafferty, I.P.; Troncoso, J.; et al. Abundant Quantitative Trait Loci Exist for DNA Methylation and Gene Expression in Human Brain. PLoS Genet. 2010, 6, e1000952. [Google Scholar] [CrossRef] [Green Version]
  70. Li, Q.; Huang, Z.; Zhao, W.; Li, M.; Li, C. Transcriptome Analysis Reveals Long Intergenic Non-Coding RNAs Contributed to Intramuscular Fat Content Differences between Yorkshire and Wei Pigs. Int. J. Mol. Sci. 2020, 21, 1732. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  71. Allfrey, V.G.; Faulkner, R.; Mirsky, A.E. Acetylation and Methylation of Histones and their Possible Role in the Regulation of RNA Synthesis. Proc. Natl. Acad. Sci. USA 1964, 51, 786–794. [Google Scholar] [CrossRef] [Green Version]
  72. Bannister, A.J.; Kouzarides, T. Regulation of chromatin by histone modifications. Cell Res. 2011, 21, 381–395. [Google Scholar] [CrossRef]
  73. Esmaeili, M.; Blythe, S.A.; Tobias, J.W.; Zhang, K.; Yang, J.; Klein, P.S. Chromatin accessibility and histone acetylation in the regulation of competence in early development. Dev. Biol. 2020, 462, 20–35. [Google Scholar] [CrossRef] [PubMed]
  74. Izzo, A.; Schneider, R. The role of linker histone H1 modifications in the regulation of gene expression and chromatin dynamics. Biochim. Biophys. Acta (BBA) Bioenerg. 2016, 1859, 486–495. [Google Scholar] [CrossRef]
  75. Martire, S.; Banaszynski, L.A. The roles of histone variants in fine-tuning chromatin organization and function. Nat. Rev. Mol. Cell Biol. 2020, 21, 1–20. [Google Scholar] [CrossRef]
  76. Xhemalce, B.; Dawson, M.A.; Bannister, A.J. Histone Modifications. In Reviews in Cell Biology and Molecular Medicine; American Cancer Society: Atlanta, GA, USA, 2011; ISBN 9783527600908. [Google Scholar]
  77. Oki, M.; Aihara, H.; Ito, T. Role of histone phosphorylation in chromatin dynamics and its implications in diseases. Subcell. Biochem. 2007, 41, 319–336. [Google Scholar] [PubMed]
  78. Bannister, A.J.; Schneider, R.; Kouzarides, T. Histone Methylation: Dynamic or Static? Cell 2002, 109, 801–806. [Google Scholar] [CrossRef] [Green Version]
  79. Copeland, R.A.; Solomon, M.E.; Richon, V.M. Protein methyltransferases as a target class for drug discovery. Nat. Rev. Drug Discov. 2009, 8, 724–732. [Google Scholar] [CrossRef]
  80. Dahl, J.A.; Reiner, A.H.; Klungland, A.; Wakayama, T.; Collas, P. Histone H3 Lysine 27 Methylation Asymmetry on Developmentally-Regulated Promoters Distinguish the First Two Lineages in Mouse Preimplantation Embryos. PLoS ONE 2010, 5, e9150. [Google Scholar] [CrossRef] [Green Version]
  81. Jambhekar, A.; Dhall, A.; Shi, Y. Roles and regulation of histone methylation in animal development. Nat. Rev. Mol. Cell Biol. 2019, 20, 625–641. [Google Scholar] [CrossRef] [PubMed]
  82. Urvalek, A.; Laursen, K.B.; Gudas, L.J. The Roles of Retinoic Acid and Retinoic Acid Receptors in Inducing Epigenetic Changes. Subcell. Biochem. 2014, 70, 129–149. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  83. Hou, N.; Ren, L.; Gong, M.; Bi, Y.; Gu, Y.; Dong, Z.; Liu, Y.; Chen, J.; Li, T. Vitamin A Deficiency Impairs Spatial Learning and Memory: The Mechanism of Abnormal CBP-Dependent Histone Acetylation Regulated by Retinoic Acid Receptor Alpha. Mol. Neurobiol. 2014, 51, 633–647. [Google Scholar] [CrossRef]
  84. Ebata, K.T.; Mesh, K.; Liu, S.; Bilenky, M.; Fekete, A.; Acker, M.G.; Hirst, M.; Garcia, B.A.; Ramalho-Santos, M. Vitamin C induces specific demethylation of H3K9me2 in mouse embryonic stem cells via Kdm3a/b. Epigenet. Chromatin 2017, 10, 1–12. [Google Scholar] [CrossRef]
  85. Andreescu, N.; Puiu, M.; Niculescu, M. Effects of Dietary Nutrients on Epigenetic Changes in Cancer. Methods Mol. Biol. 2018, 1856, 121–139. [Google Scholar] [CrossRef]
  86. Kocamis, H.; Killefer, J. Myostatin expression and possible functions in animal muscle growth. Domest. Anim. Endocrinol. 2002, 23, 447–454. [Google Scholar] [CrossRef]
  87. Liu, X.; Wang, J.; Li, R.; Yang, X.; Sun, Q.; Albrecht, E.; Zhao, R. Maternal dietary protein affects transcriptional regulation of myostatin gene distinctively at weaning and finishing stages in skeletal muscle of Meishan pigs. Epigenetics 2011, 6, 899–907. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  88. Mitani, S.; Du, H.; Hall, D.H.; Driscoll, M.; Chalfie, M. Combinatorial Control of Touch Receptor Neuron Expression in Caeno-rhabditis Elegans. Development 1993, 119, 773–783. [Google Scholar]
  89. Reinhart, B.J.; Slack, F.J.; Basson, M.; Pasquinelli, A.E.; Bettinger, J.C.; Rougvie, A.E.; Horvitz, H.R.; Ruvkun, G. The 21-nucleotide let-7 RNA regulates developmental timing in Caenorhabditis elegans. Nature 2000, 403, 901–906. [Google Scholar] [CrossRef] [PubMed]
  90. Chen, X. A MicroRNA as a Translational Repressor of APETALA2 in Arabidopsis Flower Development. Science 2004, 303, 2022–2025. [Google Scholar] [CrossRef] [Green Version]
  91. Doench, J.G. Specificity of microRNA target selection in translational repression. Genes Dev. 2004, 18, 504–511. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  92. Heneghan, H.M.; Miller, N.; Kerin, M.J. MiRNAs as biomarkers and therapeutic targets in cancer. Curr. Opin. Pharmacol. 2010, 10, 543–550. [Google Scholar] [CrossRef] [PubMed]
  93. Macfarlane, L.-A.; Murphy, P.R. MicroRNA: Biogenesis, Function and Role in Cancer. Curr. Genom. 2010, 11, 537–561. [Google Scholar] [CrossRef] [Green Version]
  94. Kim, V.N.; Han, J.; Siomi, M.C. Biogenesis of small RNAs in animals. Nat. Rev. Mol. Cell Biol. 2009, 10, 126–139. [Google Scholar] [CrossRef]
  95. German, C.A.; Shapiro, M.D. Small Interfering RNA Therapeutic Inclisiran: A New Approach to Targeting PCSK9. BioDrugs 2019, 34, 1–9. [Google Scholar] [CrossRef]
  96. Ozata, D.M.; Gainetdinov, I.; Zoch, A.; O’Carroll, D.; Zamore, P.D. PIWI-interacting RNAs: Small RNAs with big functions. Nat. Rev. Genet. 2019, 20, 89–108. [Google Scholar] [CrossRef] [Green Version]
  97. Shuwen, H.; Xi, Y.; Quan, Q.; Yin, J.; Miao, D. Can small nucleolar RNA be a novel molecular target for hepatocellular carcinoma? Gene 2020, 733, 144384. [Google Scholar] [CrossRef]
  98. Gourbault, O.; Llobat, L. MicroRNAs as Biomarkers in Canine Osteosarcoma: A New Future? Vet. Sci. 2020, 7, 146. [Google Scholar] [CrossRef] [PubMed]
  99. Nervi, C.; Grignani, F. RARs and MicroRNAs. Subcell. Biochem. 2014, 70, 151–179. [Google Scholar] [CrossRef] [PubMed]
  100. Panni, S.; Lovering, R.C.; Porras, P.; Orchard, S. Non-coding RNA regulatory networks. Biochim. Biophys. Acta (BBA) Bioenerg. 2020, 1863, 194417. [Google Scholar] [CrossRef]
  101. Bravo, J.I.; Nozownik, S.; Danthi, P.S.; Benayoun, B.A. Transposable elements, circular RNAs and mitochondrial transcription in age-related genomic regulation. Development 2020, 147. [Google Scholar] [CrossRef]
  102. Kumar, S.; Gonzalez, E.A.; Rameshwar, P.; Etchegaray, J.-P. Non-Coding RNAs as Mediators of Epigenetic Changes in Malignancies. Cancers 2020, 12, 3657. [Google Scholar] [CrossRef] [PubMed]
  103. Castel, S.E.; Martienssen, R.A. RNA interference in the nucleus: Roles for small RNAs in transcription, epigenetics and beyond. Nat. Rev. Genet. 2013, 14, 100–112. [Google Scholar] [CrossRef] [PubMed]
  104. Kiss-László, Z.; Henry, Y.; Bachellerie, J.-P.; Caizergues-Ferrer, M.; Kiss, T. Site-Specific Ribose Methylation of Preribosomal RNA: A Novel Function for Small Nucleolar RNAs. Cell 1996, 85, 1077–1088. [Google Scholar] [CrossRef] [Green Version]
  105. Ni, J.; Tien, A.L.; Fournier, M.J. Small Nucleolar RNAs Direct Site-Specific Synthesis of Pseudouridine in Ribosomal RNA. Cell 1997, 89, 565–573. [Google Scholar] [CrossRef] [Green Version]
  106. Naeli, P.; Pourhanifeh, M.H.; Karimzadeh, M.R.; Shabaninejad, Z.; Movahedpour, A.; Tarrahimofrad, H.; Mirzaei, H.R.; Bafrani, H.H.; Savardashtaki, A.; Mirzaei, H.; et al. Circular RNAs and gastrointestinal cancers: Epigenetic regulators with a prognostic and therapeutic role. Crit. Rev. Oncol. 2020, 145, 102854. [Google Scholar] [CrossRef]
  107. Meng, S.; Zhou, H.; Feng, Z.; Xu, Z.; Tang, Y.; Wu, M. Epigenetics in Neurodevelopment: Emerging Role of Circular RNA. Front. Cell. Neurosci. 2019, 13, 327. [Google Scholar] [CrossRef]
  108. Aravin, A.A.; Sachidanandam, R.; Girard, A.; Fejes-Toth, K.; Hannon, G.J. Developmentally Regulated piRNA Clusters Implicate MILI in Transposon Control. Science 2007, 316, 744–747. [Google Scholar] [CrossRef] [Green Version]
  109. Watanabe, T.; Tomizawa, S.-I.; Mitsuya, K.; Totoki, Y.; Yamamoto, Y.; Kuramochi-Miyagawa, S.; Iida, N.; Hoki, Y.; Murphy, P.J.; Toyoda, A.; et al. Role for piRNAs and Noncoding RNA in de Novo DNA Methylation of the Imprinted Mouse Rasgrf1 Locus. Science 2011, 332, 848–852. [Google Scholar] [CrossRef] [Green Version]
  110. Iyer, M.K.; Niknafs, Y.S.; Malik, R.; Singhal, U.; Sahu, A.; Hosono, Y.; Barrette, T.R.; Prensner, J.R.; Evans, J.R.; Zhao, S.; et al. The landscape of long noncoding RNAs in the human transcriptome. Nat. Genet. 2015, 47, 199–208. [Google Scholar] [CrossRef]
  111. Gupta, R.A.; Shah, N.; Wang, K.C.; Kim, J.; Horlings, H.M.; Wong, D.J.; Tsai, M.-C.; Hung, T.; Argani, P.; Rinn, J.L.; et al. Long non-coding RNA HOTAIR reprograms chromatin state to promote cancer metastasis. Nat. Cell Biol. 2010, 464, 1071–1076. [Google Scholar] [CrossRef]
  112. Rinn, J.L.; Kertesz, M.; Wang, J.K.; Squazzo, S.L.; Xu, X.; Brugmann, S.A.; Goodnough, L.H.; Helms, J.A.; Farnham, P.J.; Segal, E.; et al. Functional Demarcation of Active and Silent Chromatin Domains in Human HOX Loci by Noncoding RNAs. Cell 2007, 129, 1311–1323. [Google Scholar] [CrossRef] [Green Version]
  113. Amanzadeh, J.; Gitomer, W.L.; Zerwekh, J.E.; Preisig, P.A.; Moe, O.W.; Pak, C.Y.C.; Levi, M. Effect of high protein diet on stone-forming propensity and bone loss in rats. Kidney Int. 2003, 64, 2142–2149. [Google Scholar] [CrossRef] [Green Version]
  114. Rosenberg, M.E.; Chmielewski, D.; Hostetter, T.H. Effect of dietary protein on rat renin and angiotensinogen gene expression. J. Clin. Investig. 1990, 85, 1144–1149. [Google Scholar] [CrossRef] [PubMed]
  115. Kato, S.; Takeyama, K.-I.; Kojima, R.; Yoshizawa, Y.; Furusho, T.; Mano, H.; Masushige, S. Gene Expression of Cellular Retinol-Binding Protein I (CRBP I) is Affected by Dietary Proteins in the Rat Liver. J. Nutr. Sci. Vitaminol. 1993, 39, 545–554. [Google Scholar] [CrossRef]
  116. Endo, Y.; Fu, Z.; Abe, K.; Arai, S.; Kato, H. Dietary Protein Quantity and Quality Affect Rat Hepatic Gene Expression. J. Nutr. 2002, 132, 3632–3637. [Google Scholar] [CrossRef] [PubMed]
  117. Cervantes-Pahm, S.K.; Stein, H.H. Ileal digestibility of amino acids in conventional, fermented, and enzyme-treated soybean meal and in soy protein isolate, fish meal, and casein fed to weanling pigs. J. Anim. Sci. 2010, 88, 2674–2683. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  118. Imam, S.; Yagi, I.; Saeki, T.; Kotaru, M.; Iwami, K. Quantity as Well as Quality of Dietary Protein Affects Serine Dehydratase Gene Expression in Rat Liver. J. Nutr. Sci. Vitaminol. 2003, 49, 33–39. [Google Scholar] [CrossRef] [Green Version]
  119. Gheorghe, C.P.; Goyal, R.; Holweger, J.D.; Longo, L.D. Placental Gene Expression Responses to Maternal Protein Restriction in the Mouse. Placenta 2009, 30, 411–417. [Google Scholar] [CrossRef] [Green Version]
  120. Altobelli, G.; Bogdarina, I.G.; Stupka, E.; Clark, A.J.L.; Langley-Evans, S. Genome-Wide Methylation and Gene Expression Changes in Newborn Rats following Maternal Protein Restriction and Reversal by Folic Acid. PLoS ONE 2013, 8, e82989. [Google Scholar] [CrossRef] [PubMed]
  121. Altmann, S.; Muràni, E.; Schwerin, M.; Metges, C.C.; Wimmers, K.; Ponsuksili, S. Maternal dietary protein restriction and excess affects offspring gene expression and methylation of non-SMC subunits of condensin I in liver and skeletal muscle. Epigenetics 2012, 7, 239–252. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  122. Altmann, S.; Muràni, E.; Schwerin, M.; Metges, C.C.; Wimmers, K.; Ponsuksili, S. Dietary protein restriction and excess of pregnant German Landrace sows induce changes in hepatic gene expression and promoter methylation of key metabolic genes in the offspring. J. Nutr. Biochem. 2013, 24, 484–495. [Google Scholar] [CrossRef]
  123. Cong, R.; Jia, Y.; Li, R.; Ni, Y.; Yang, X.; Sun, Q.; Parvizi, N.; Zhao, R. Maternal low-protein diet causes epigenetic deregulation of HMGCR and CYP7α1 in the liver of weaning piglets. J. Nutr. Biochem. 2012, 23, 1647–1654. [Google Scholar] [CrossRef]
  124. Wan, X.; Wang, S.; Xu, J.; Zhuang, L.; Xing, K.; Zhang, M.; Zhu, X.; Wang, L.; Gao, P.; Xi, Q.; et al. Dietary protein-induced hepatic IGF-1 secretion mediated by PPARγ activation. PLoS ONE 2017, 12, e0173174. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  125. Rehfeldt, C.; Lang, I.S.; Görs, S.; Hennig, U.; Kalbe, C.; Stabenow, B.; Brüssow, K.-P.; Pfuhl, R.; Bellmann, O.; Nürnberg, G.; et al. Limited and excess dietary protein during gestation affects growth and compositional traits in gilts and impairs offspring fetal growth. J. Anim. Sci. 2011, 89, 329–341. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  126. Rehfeldt, C.; Stabenow, B.; Pfuhl, R.; Block, J.; Nürnberg, G.; Otten, W.; Metges, C.C.; Kalbe, C. Effects of limited and excess protein intakes of pregnant gilts on carcass quality and cellular properties of skeletal muscle and subcutaneous adipose tissue in fattening pigs. J. Anim. Sci. 2012, 90, 184–196. [Google Scholar] [CrossRef]
  127. DelCurto, H.; Wu, G.; Satterfield, M.C. Nutrition and reproduction: Links to Epigenetics and Metabolic Syndrome in Offspring. Curr. Opin. Clin. Nutr. Metab. Care 2013, 16, 385–391. [Google Scholar] [CrossRef]
  128. Bestor, T.H. The DNA methyltransferases of mammals. Hum. Mol. Genet. 2000, 9, 2395–2402. [Google Scholar] [CrossRef] [Green Version]
  129. Ji, Y.; Nordgren, K.K.S.; Chai, Y.; Hebbring, S.J.; Jenkins, G.D.; Abo, R.P.; Peng, Y.; Pelleymounter, L.L.; Moon, I.; Eckloff, B.W.; et al. Human Liver Methionine Cycle: MAT1A and GNMT Gene Resequencing, Functional Genomics, and Hepatic Genotype-Phenotype Correlation. Drug Metab. Dispos. 2012, 40, 1984–1992. [Google Scholar] [CrossRef] [Green Version]
  130. Cai, D.; Wang, J.; Jia, Y.; Liu, H.; Yuan, M.; Dong, H.; Zhao, R. Gestational dietary betaine supplementation suppresses hepatic expression of lipogenic genes in neonatal piglets through epigenetic and glucocorticoid receptor-dependent mechanisms. Biochim. Biophys. Acta (BBA) Mol. Cell Biol. Lipids 2016, 1861, 41–50. [Google Scholar] [CrossRef]
  131. Cai, D.; Yuan, M.; Jia, Y.; Liu, H.; Hu, Y.; Zhao, R. Maternal gestational betaine supplementation-mediated suppression of hepatic cyclin D2 and presenilin1 gene in newborn piglets is associated with epigenetic regulation of the STAT3-dependent pathway. J. Nutr. Biochem. 2015, 26, 1622–1631. [Google Scholar] [CrossRef] [PubMed]
  132. Li, X.; Sun, Q.; Li, X.; Cai, D.; Sui, S.; Jia, Y.; Song, H.; Zhao, R. Dietary betaine supplementation to gestational sows enhances hippocampal IGF2 expression in newborn piglets with modified DNA methylation of the differentially methylated regions. Eur. J. Nutr. 2014, 54, 1201–1210. [Google Scholar] [CrossRef]
  133. Naderi, N.; House, J.D. Recent Developments in Folate Nutrition. Adv. Food Nutr. Res. 2018, 83, 195–213. [Google Scholar] [CrossRef]
  134. Robinson, J.L.; McBreairty, L.E.; Randell, E.W.; Harding, S.V.; Bartlett, R.K.; Brunton, J.A.; Bertolo, R.F. Betaine or folate can equally furnish remethylation to methionine and increase transmethylation in methionine-restricted neonates. J. Nutr. Biochem. 2018, 59, 129–135. [Google Scholar] [CrossRef] [Green Version]
  135. He, Q.; Zou, T.; Chen, J.; Jian, L.; He, J.; Xia, Y.; Xie, F.; Wang, Z.; You, J. Maternal Methyl-Donor Micronutrient Supplementation During Pregnancy Promotes Skeletal Muscle Differentiation and Maturity in Newborn and Weaning Pigs. Front. Nutr. 2020, 7, 609022. [Google Scholar] [CrossRef]
  136. Navik, U.; Sheth, V.G.; Kabeer, S.W.; Tikoo, K. Dietary Supplementation of Methyl Donor L-Methionine Alters Epigenetic Modification in Type 2 Diabetes. Mol. Nutr. Food Res. 2019, 63, e1801401. [Google Scholar] [CrossRef]
  137. Batistel, F.; Alharthi, A.S.; Yambao, R.R.C.; A Elolimy, A.; Pan, Y.-X.; Parys, C.; Loor, J.J. Methionine Supply During Late-Gestation Triggers Offspring Sex-Specific Divergent Changes in Metabolic and Epigenetic Signatures in Bovine Placenta. J. Nutr. 2019, 149, 6–17. [Google Scholar] [CrossRef] [PubMed]
  138. Van Riet, M.M.J.; Millet, S.; Langendries, K.C.M.; Van Zelst, B.D.; Janssens, G.P.J. Association between methylation potential and nutrient metabolism throughout the reproductive cycle of sows. J. Anim. Physiol. Anim. Nutr. 2019, 103, 858–867. [Google Scholar] [CrossRef] [PubMed]
  139. Biggar, K.K.; Li, S.S.-C. Non-histone protein methylation as a regulator of cellular signalling and function. Nat. Rev. Mol. Cell Biol. 2015, 16, 5–17. [Google Scholar] [CrossRef]
  140. Bidner, B.; Ellis, M.; Witte, D.; Carr, S.; McKeith, F. Influence of dietary lysine level, pre-slaughter fasting, and rendement napole genotype on fresh pork quality. Meat Sci. 2004, 68, 53–60. [Google Scholar] [CrossRef]
  141. Witte, D.P.; Ellis, M.; McKeith, F.K.; Wilson, E.R. Effect of dietary lysine level and environmental temperature during the finishing phase on the intramuscular fat content of pork. J. Anim. Sci. 2000, 78, 1272–1276. [Google Scholar] [CrossRef] [Green Version]
  142. He, L.; Yang, H.; Hou, Y.; Li, T.; Fang, J.; Zhou, X.; Yin, Y.; Wu, L.; Nyachoti, M.; Wu, G. Effects of dietary l-lysine intake on the intestinal mucosa and expression of CAT genes in weaned piglets. Amino Acids 2013, 45, 383–391. [Google Scholar] [CrossRef] [PubMed]
  143. Morales, A.; Garcia, H.; Arce, N.; Cota, M.; Zijlstra, R.T.; Araiza, B.A.; Cervantes, M. Effect of L-lysine on expression of selected genes, serum concentration of amino acids, muscle growth and performance of growing pigs. J. Anim. Physiol. Anim. Nutr. 2014, 99, 701–709. [Google Scholar] [CrossRef]
  144. Katsumata, M.; Kawakami, S.; Kaji, Y.; Takada, R.; Dauncey, M.J. Differential Regulation of Porcine Hepatic IGF-I mRNA Expression and Plasma IGF-I Concentration by a Low Lysine Diet. J. Nutr. 2002, 132, 688–692. [Google Scholar] [CrossRef] [Green Version]
  145. Liao, S.F.; Wang, T.; Regmi, N. Lysine nutrition in swine and the related monogastric animals: Muscle protein biosynthesis and beyond. SpringerPlus 2015, 4, 147. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  146. Rajantie, J.; Simell, O.; Rapola, J.; Perheentupa, J. Lysinuric protein intolerance: A two-year trial of dietary supplementation therapy with citrulline and lysine. J. Pediatr. 1980, 97, 927–932. [Google Scholar] [CrossRef]
  147. Saudubray, J.-M.; Rabier, D. Biomarkers identified in inborn errors for lysine, arginine, and ornithine. J. Nutr. 2007, 137, 1669S–1672S. [Google Scholar] [CrossRef] [Green Version]
  148. Edmonds, M.S.; Baker, D.H. Failure of Excess Dietary Lysine to Antagonize Arginine in Young Pigs. J. Nutr. 1987, 117, 1396–1401. [Google Scholar] [CrossRef] [PubMed]
Figure 1. Current recommendations of crude protein (A), digestible lysine (B), and digestible methionine (C) of the different physiological phases of pig production [30,31,32].
Figure 1. Current recommendations of crude protein (A), digestible lysine (B), and digestible methionine (C) of the different physiological phases of pig production [30,31,32].
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Figure 2. Scheme of the regulation of gene expression by DNA methylation. Methyl groups were added by DMNT1, DNMT3a, and DNMT3b enzymes in cytosine of CpG island. As result, the RNA polymerase is unable to bind to DNA sequence, and the gene promoter is not expressed.
Figure 2. Scheme of the regulation of gene expression by DNA methylation. Methyl groups were added by DMNT1, DNMT3a, and DNMT3b enzymes in cytosine of CpG island. As result, the RNA polymerase is unable to bind to DNA sequence, and the gene promoter is not expressed.
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Figure 3. Scheme of the regulation of gene expression by histone modifications. Enzymes as histone methyltransferase and acetyltransferase add or remove methyl, acetyl, and phosphate groups of histones, influencing to transcriptional machinery, and they activate or repress gene expression by de-condensing or condensing chromatin, respectively.
Figure 3. Scheme of the regulation of gene expression by histone modifications. Enzymes as histone methyltransferase and acetyltransferase add or remove methyl, acetyl, and phosphate groups of histones, influencing to transcriptional machinery, and they activate or repress gene expression by de-condensing or condensing chromatin, respectively.
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Figure 4. Diagram of miRNA biogenesis. In the nucleus, miRNA that are transcribed by RNA polymerase II or III as primary transcripts (pri-miRNA). The enzyme Drosha and its cofactor DGR8/Pasha then cut the pri-miRNA molecule, to form a pre-miRNA. This pre-miRNA is actively transported from the nucleus to the cytoplasm by the nuclear transport receptor Exportin 5 (XPO5) in a Ran-GTP-protein-dependent manner by XPO5. In the cytoplasm, the pre-miRNA is cut by a second enzyme, called Dicer, until the formation of a mature and short double-stranded miRNA molecule. The miRNA duplex unwinds and is incorporated into the RNA induced silencing complex (RISC) protein [98].
Figure 4. Diagram of miRNA biogenesis. In the nucleus, miRNA that are transcribed by RNA polymerase II or III as primary transcripts (pri-miRNA). The enzyme Drosha and its cofactor DGR8/Pasha then cut the pri-miRNA molecule, to form a pre-miRNA. This pre-miRNA is actively transported from the nucleus to the cytoplasm by the nuclear transport receptor Exportin 5 (XPO5) in a Ran-GTP-protein-dependent manner by XPO5. In the cytoplasm, the pre-miRNA is cut by a second enzyme, called Dicer, until the formation of a mature and short double-stranded miRNA molecule. The miRNA duplex unwinds and is incorporated into the RNA induced silencing complex (RISC) protein [98].
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Figure 5. Schematic explanation of one-carbon unit metabolism. Methyl donors participate in the transfer of one-carbon units for the methylation reactions. The enzymes related with pathways are (1) choline dehydrogenase, (2) betaine homocysteine methyltransferase, (3) methionine synthase, (4) S-adenosylmethionine synthase, and (5) S-adenosylmethionine synthase. SAH, S-adenosylhomocysteine; SAM, S-adenosylmethionine.
Figure 5. Schematic explanation of one-carbon unit metabolism. Methyl donors participate in the transfer of one-carbon units for the methylation reactions. The enzymes related with pathways are (1) choline dehydrogenase, (2) betaine homocysteine methyltransferase, (3) methionine synthase, (4) S-adenosylmethionine synthase, and (5) S-adenosylmethionine synthase. SAH, S-adenosylhomocysteine; SAM, S-adenosylmethionine.
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Table 1. Different non-coding RNAs related to epigenetics.
Table 1. Different non-coding RNAs related to epigenetics.
Non-Coding RNAFunctionsReferences
Small Interfering RNA (siRNA)Gene silencing[103]
Small Nucleolar RNA (snoRNA)rRNA modifications[104,105]
Circular RNA (circRNA)miRNA sponge, regulation of gene transcription, RNA binding protein sponge[106,107]
Piwi-interacting RNA (piRNA)Transposon repression, DNA methylation[108,109]
Long Non-coding RNA (lncRNA)X-chromosome inactivation, telomere regulation, imprinting[110,111,112]
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Marín-García, P.J.; Llobat, L. How Does Protein Nutrition Affect the Epigenetic Changes in Pig? A Review. Animals 2021, 11, 544. https://doi.org/10.3390/ani11020544

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Marín-García PJ, Llobat L. How Does Protein Nutrition Affect the Epigenetic Changes in Pig? A Review. Animals. 2021; 11(2):544. https://doi.org/10.3390/ani11020544

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Marín-García, Pablo Jesús, and Lola Llobat. 2021. "How Does Protein Nutrition Affect the Epigenetic Changes in Pig? A Review" Animals 11, no. 2: 544. https://doi.org/10.3390/ani11020544

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