Skip to main content

REVIEW article

Front. Vet. Sci., 19 July 2024
Sec. Animal Nutrition and Metabolism

Exploring the potential roles of apelin, visfatin, and irisin in energy regulation in farm animals: an overview

Borhan Shokrollahi
Borhan Shokrollahi1*Sun-Sik JangSun-Sik Jang2Hyun Jeong LeeHyun Jeong Lee2Hafiz Ishfaq AhmadHafiz Ishfaq Ahmad3Abdul Rahman SesayAbdul Rahman Sesay4Ali Ghazikhani ShadAli Ghazikhani Shad5Salim MorammaziSalim Morammazi6Sameh A. AbdelnourSameh A. Abdelnour7
  • 1Department of Animal Science, Sanandaj Branch, Islamic Azad University, Sanandaj, Iran
  • 2Animal Nutrition and Physiology Division, National Institute of Animal Science, Rural Development Administration, Wanju-gun, Republic of Korea
  • 3Department of Animal Breeding and Genetics, University of Veterinary and Animal Sciences, Pattoki, Pakistan
  • 4Department of Animal Science, Njala University, Bo, Sierra Leone
  • 5Department of Animal Science, Saveh Branch, Islamic Azad University, Saveh, Iran
  • 6Department of Animal Science, Faculty of Agricultural and Natural Resources, Persian Gulf University, Bushehr, Iran
  • 7Department of Animal Production, Faculty of Agriculture, Zagazig University, Zagazig, Egypt

Adipose tissue, both intricate and fundamental to physiological functions, comprises cell types, including adipocytes, pivotal in secreting bioactive peptides known as ‘adipokines.’ Apelin (APLN), Visfatin (VSFTN), and Irisin (IRSN) are novel adipokines involved in regulating energy, carbohydrate, protein, and lipid metabolism. APLN acts as an endogenous ligand for G-protein-coupled receptors, VSFTN is essential in nicotinamide adenine dinucleotide (NAD) biosynthesis, and IRSN is released from skeletal muscle and adipose tissues. Their influence spans various physiological domains, including insulin resistance and sensitivity, cardiovascular functions, angiogenesis, and reproductive systems. This review focuses on the potential roles of APLN, VSFTN, and IRSN in energy regulation mechanisms related to farm animal production. Despite accumulating evidence of their significance, comprehensive understanding is still emerging, with most studies based on model organisms. Thus, there’s a pressing need for targeted research on farm animals. Addressing these knowledge gaps could pave the way for improved health strategies, reproductive efficiency, and productivity in farm animals. Future research should focus on understanding the multifaceted interactions of these adipokines and their implications for promoting sustainable and effective animal production.

1 Introduction

Adipose tissue (AT) is not merely a lipid-storage compartment but a complex endocrine organ with significant metabolic functionality (1). It mediates numerous physiological processes, including neuroendocrine modulation, energetic homeostasis, immunological activities, macrophage reconfiguration, and reproductive functions (2). Historically, AT has been classified into three principal categories: white AT (WAT), brown AT (BAT), and beige AT (BeAT) (3). WAT, which is widely distributed throughout the human body, includes mature adipocytes, macrophages, fibroblasts, endothelial cells, and preadipocytes, all playing integral roles in various energetic homeostasis pathways (1, 4). Conversely, BAT is specialized in energy expenditure, contrasting with WAT’s energy storage function. BAT’s distinguishing features include a high content of lipid droplets and an abundance of mitochondria, which facilitate its role in thermogenesis (5).

Notably, WAT secretes a wide array of bioactive peptides, including both anti-inflammatory and pro-inflammatory factors. These peptides, known as ‘adipokines’ or ‘cytokines,’ have diverse roles, such as modulating energetic homeostasis, regulating reproductive processes, adjusting metabolic balance, and being linked to various cardiovascular pathologies associated with adiposity (6). Key adipokines include leptin (LEP), Retinol Binding Protein 4 (RBP4), and adiponectin (ADIPOQ) (7).

While adiponectin and leptin are renowned for their involvement in energy regulation (8), emerging adipokines, notably APLN, VSFTN, and IRSN, reveal their significance in energy metabolism. APLN, an endogenous ligand of the APJ, a member of the orphan G-protein-coupled receptor (GPCR) family, closely resembles the angiotensin-II receptor (9). Fluctuations in the plasma levels of APLN are observed with weight variations, associating it directly with obesity (10). APLN also shows potential in modulating insulin sensitivity and cardiovascular functions (11).

VSFTN, also known as pre-B cell colony-enhancing factor 1 (PBEF1) or Nicotinamide phosphoribosyltransferase (NAMPT), is involved in B-cell maturation and neutrophil apoptosis (12). Predominantly found in visceral AT (13), several studies have explored its correlation with obesity and type 2 diabetes (14).

IRSN, a notable myokine and adipocytokine, functions across various tissues (15). It can upregulate the expression of uncoupling protein 1 (UCP1) in mitochondria, with its levels influenced by diet, exercise, obesity, and pharmacological agents (16, 17).

In farm animals, adipokines such as APLN, VSFTN, and IRSN are crucial for modulating nutrient intake, energy flux, and maintaining metabolic homeostasis (18). These mechanisms are especially important in livestock facing challenges related to negative energy balance (NEB) (19). The literature highlights the impact of these adipokines on various physiological processes, including metabolic dysregulations, angiogenesis, lipid homeostasis, and adiposity. Additionally, they have diverse effects on the mammalian reproductive system (20).

Despite their significance across multiple species, there is a notable gap in understanding their specific roles in the energy metabolism of farm animals. This review aims to investigate the structures, functions, and potential applications of APLN, VSFTN, and IRSN across different species, with a particular focus on farm animals. By comparing their known roles in other species, we emphasize the urgent need for targeted studies on these adipokines in livestock to enhance energy metabolism and production.

2 APLN isoforms, gene localization, and molecular interactions

APLN, recognized as an endogenous ligand, uniquely binds to the APLN receptor (APJ) (21). It originates from APLN-77 or pre-pro-APLN. A spectrum of APLN isoforms emerge from it, including APLN-36, APLN-19, APLN-17, APLN-13, and APLN-12 (2224). These isoforms are derived from the C-terminal of the preproprotein (25, 26). APLN-36 is considered the mature peptide due to its alignment with the 36\u00B0C-terminal amino acids (AAs) of the pre-pro-APLN protein (25). The conserved C-terminal 17 AA sequence, labeled as APLN-17 or K17F, includes APLN-13 (9, 25). Alterations in APLN-13’s N-terminal glutamine result in pyroglutamyl formations, highlighting significant APLN molecular structures (27).

2.1 Gene localization

The APLN gene is located on chromosome Xq25-26.1 in humans, marked by a single intron around 6 kb long (9, 28). In rats and mice, the gene is positioned at Xq35 and XA3.2, respectively (9). Identified primary promoter regions include-207/−1 for rats and-100/+74 base pairs for humans (29). A significant similarity of 76–95% is observed among bovine, human, rat, and mouse pre-pro-APLN precursors, with each species believed to possess a native dimeric APLN protein form (30).

2.2 APJ receptor

APJ, also designated as APLNR, belongs to the seven-transmembrane G-protein coupled receptors (GPCRs) family, specifically within the Rhodopsin-like GPCRs class (31). Its sequence comprises 380 AAs, and its nomenclature is driven by the interaction with its ligand, APLN (32).

2.3 Molecular conformation

Although a definitive APLN structure is absent in the Protein Data Bank (PDB), available studies report that APLN-13 and APLN-36 adopt a “random conformation” at ambient temperatures (33). Circular dichroism spectroscopy (CD) studies indicate a random coil conformation for various APLN isoforms at 5°C and 35°C. APLN-17 is characterized by dominant β-turns and polyproline-II (PPII) structures spanning its peptide configuration (24, 26).

2.4 Expression and function

APLN mRNA is detected in stromal-vascular cells and adipocytes (34). However, its expression remains stable across intraabdominal and subcutaneous fat tissues (10). A key functional aspect of APLN is its activation of the Gi/Gq pathways, modulating intracellular AMP concentrations and inhibiting isoproterenol-induced lipolysis among other pathways (Figure 1). Exploring APLN’s structural and functional nuances can illuminate its potential implications in energy regulation within farm animals.

Figure 1
www.frontiersin.org

Figure 1. APLN, a GPCR ligand, activates Gi/Gq pathways to modulate intracellular AMPR concentration and inhibit isoproterenol-induced lipolysis, initiating other pathways.

3 APLN’s distribution and its integral role in glucose homeostasis and insulin sensitivity

3.1 Distribution

APLN is ubiquitous in both humans’ and rats’ central nervous system (CNS) and peripheral tissues (35). It is detected in various organs, such as the testicles, intestines, and fetus, with variable expression levels across the placenta, heart, lungs, kidneys, and vascular endothelial cells (3638). Distinctly, APLN expression is pronounced across adipose, connective, and vascular smooth muscle cells (36). Additionally, its presence spans various fish tissues, encompassing the brain, pituitary, spleen, kidney, and liver (3941). In sheep, APLN is also expressed in peripheral organs such as the mammary gland, abomasum, and duodenum, in addition to the uterus (4244).

3.2 Role in glucose homeostasis

Central APLN’s relevance is undeniable. Several CNS nuclei exhibit APLN mRNA, indicating its role in glucose metabolism (45). Specifically, APLN-positive nerve fibers in the hypothalamus point to APLN-producing neurons that modulate glucose homeostasis, influenced by circulating peptides and neurotransmitters (46). Numerous studies have solidified APLN’s critical role in insulin sensitivity and glucose metabolism. For instance, during conditions that inhibit hepatic glucose production, APLN fosters decreased blood glucose levels by enhancing glucose uptake in skeletal muscles and ATs, ultimately boosting insulin sensitivity (47, 48). Mechanistically, APLN promotes glucose transport in muscles and modulates pathways involving AMP-activated protein kinase (AMPK) and endothelial nitric oxide synthase (eNOS) (11, 48). AMPK activation in muscle cells is pivotal for APLN-induced glucose uptake (49). APLN also enhances glucose movement from the intestinal lumen to the bloodstream, influencing glucose levels in the portal vein and insulin production and sensitivity (36, 50).

3.3 Findings in dairy cows

Notably, studies on dairy cow reveal contrasting findings on APLN levels post-calving. One study observed decreased APLN levels after calving, with linked fluctuations in insulin and glucose concentrations (51). In contrast, another study reported consistent APLN levels during the transition from pregnancy to lactation (52).

APLN’s widespread distribution and its integral role in glucose metabolism and insulin sensitivity emphasize its potential importance in farm animal health, especially dairy cows. Monitoring APLN fluctuations might be key to optimizing these animals’ metabolic health and energy balance, particularly during pivotal stages such as pregnancy-to-lactation transition.

For a visual representation of the aforementioned mechanisms, Figure 2 offers a detailed schematic overview.

Figure 2
www.frontiersin.org

Figure 2. APLN enhances glucose uptake in skeletal muscles, ATs, and myocytes to maintain low blood glucose levels.

4 APLN’s multifaceted impact on lipid regulation and systemic metabolic functions

4.1 Energy homeostasis

Energy homeostasis and nutrient metabolism are harmonized by a synergy of paracrine, endocrine, and autocrine regulators. Vital organs like the liver, pancreatic β-cells, AT, and skeletal muscle orchestrate this balance (53). Imbalances may usher in conditions like obesity, often linked with insulin resistance. Increased plasma APLN concentrations have been associated with obesity and type 2 diabetes (48).

4.2 Lipid regulation

APLN counteracts isoproterenol-induced lipolysis in isolated and differentiated 3 T3-L1 adipocytes (54). This modulation leverages the GQ, Gi, and AMPK signaling pathways, crucial for orchestrating cellular metabolic responses (55). By inhibiting lipid catabolism in adipocytes, APLN limits the release of free fatty acids. This is achieved through AMPK activation and the upsurge in perilipin surrounding lipid vacuoles, shielding stored lipids from lipase activity (54). APLN also fosters insulin secretion and enhances mitochondrial biogenesis in skeletal muscles and cardiomyocytes, increasing mitochondrial density and efficiency (56, 57).

4.3 Role in angiogenesis and fluid homeostasis

APLN promotes endothelial cell proliferation, migration, and neovascularization (45). In the hypothalamus, APLN regulates the secretion of antidiuretic hormone (ADH), essential for fluid homeostasis (58). It also triggers α-MSH release, a neuropeptide known to reduce food consumption, potentially offsetting metabolic disparities in obese subjects despite receptor desensitization (59). APLN and its receptor, APJ, play roles in water metabolism, synergizing with ADH to maintain fluid balance (36).

4.4 Implications for farm animals

APLN’s role in lipid and broader metabolic processes highlights its potential significance for livestock metabolic health. By influencing lipid metabolism, enhancing mitochondrial activity, and promoting angiogenesis, APLN could be pivotal in optimizing livestock productivity and overall health.

A summary of APLN’s metabolic impacts, as documented in reported findings from different species, is presented in Table 1.

Table 1
www.frontiersin.org

Table 1. Biological effects of APLN in animals: a summary of findings.

5 Diverse signaling pathways and physiological impacts of APLN in metabolic regulation

5.1 Signaling pathways

APLN modulates a host of cellular activities through distinct signaling pathways, notably activating AMPK, which reduces the release of free fatty acids (FFA) from 3 T3-L1 adipocytes by enhancing lipoprotein stability (70). Isoforms of APLN, including APLN-36, APLN-13, APLN-17, and [pyr1]-APLN-13, inhibit forskolin-induced cAMP production via the Gαi/o protein in the APLN/APJ system, blocking specific PKA pathway effects (36, 71).

APLN also stimulates glucose transport in human AT explants through the AMPK pathway, while in 3 T3-L1 adipocytes, it enhances glucose transport via the PI3K/Akt signaling pathway (72, 73). Additionally, APLN boosts insulin-stimulated glucose transport in insulin-resistant 3 T3-L1 cells (73).

5.2 Physiological impacts

APLN regulates various physiological functions, including blood pressure, energy metabolism, blood flow, hydration, food intake, and immune function (28). It induces nitric oxide (NO) release, leading to vasorelaxation and increased heart muscle contractility (74). APLN also directs endothelial cell chemotaxis and provides anti-apoptotic protection (75). Its interaction with appetite-regulating hormones, such as orexin, highlights its role in complex metabolic networks (76, 77). In sheep, APLN expression has been identified in various peripheral organs, including the mammary gland, abomasum, and duodenum, in addition to the uterus. This widespread distribution suggests that APLN may play multiple roles in energy regulation and reproductive functions in sheep (42). For instance, the presence of APLN in the mammary gland could be associated with lactation and milk production processes. Similarly, its expression in the abomasum and duodenum indicates a potential role in digestive processes and nutrient absorption (43, 44). Further research is necessary to explore these roles and their implications for sheep health and productivity.

5.3 Implications for farm animals

Understanding APLN’s multifaceted roles is crucial for energy regulation in farm animals. APLN’s effects on glucose and lipid metabolism, alongside its broader physiological impacts, suggest potential strategies for optimizing energy balance, health, and productivity in livestock. Further research on APLN’s signaling pathways could lead to innovative animal management and health applications.

6 Molecular insights and pervasive impact of VSFTN across species and tissues

6.1 Identification and structure

VSFTN, initially identified as the pre-B cell colony-enhancing factor (PBEF), is characterized by its 52 kDa molecular weight and 491 amino acids (AAs), which are highly conserved across species (78). The porcine VSFTN gene is located on chromosome SSC9, sharing structural similarities with the human counterpart (13, 79). It plays a crucial role in the nicotinamide adenine dinucleotide (NAD) biosynthesis pathway and is also known as Nicotinamide Phosphoribosyltransferase (NAMPT) (80, 81).

6.2 Forms and localization

NAMPT exists in two forms: intracellular (iNAMPT) and extracellular (eNAMPT) (82). iNAMPT is predominantly found in BAT and less in WAT, while eNAMPT is expressed in various cells, including adipocytes, myocytes, neurons, and immune cells (83, 84). iNAMPT is also present in the liver, kidneys, heart, skeletal muscle, and brain (20). eNAMPT, on the other hand, is expressed across a diverse array of cells ranging from adipocytes and myocytes to neurons and immune cells (83).

6.3 Structural organization

VSFTN’s monomer is organized into three domains: A, B, and C, each characterized by specific arrangements of α-helices and β-strands (7). Domain A features an antiparallel seven-stranded β-sheet/core flanked by five helices, domain B has another seven-stranded β-sheet/core, and domain C presents a simpler three-stranded β-sheet in an antiparallel configuration (7).

6.4 Functional role

VSFTN is integral to NAD biosynthesis and influences pancreatic beta-cell functions (85). As NAMPT, it catalyzes the transformation of nicotinamide into nicotinamide mononucleotide (NMN), a crucial precursor for NAD synthesis. In pancreatic beta cells, this enhances glucose-stimulated insulin secretion through sirtuin-1 activation, a NAD-dependent deacetylase, regulating glucose-responsive insulin secretion (86).

6.5 Pervasive presence

VSFTN is detected in diverse human and animal tissues, such as AT, muscle, heart, and bone marrow (87). It has homologs in organisms ranging from mollusks and bacteria to mammals. In mice, VSFTN is located in the hypothalamus and certain pituitary lobes (88). Additionally, there are gender and tissue-specific variations in VSFTN mRNA expression among broiler chickens, indicating its responsiveness to energy balance-related determinants (89).

6.6 Implications for farm animals

Given its central role in energy regulation, particularly in NAD synthesis and insulin secretion, VSFTN is pivotal for understanding energy balance in farm animals. Its widespread presence across multiple species and organs suggests that deeper exploration into VSFTN’s mechanisms could unveil strategies to enhance health, metabolic efficiency, and overall productivity in livestock.

7 VSFTN’s multifaceted impact: from metabolic regulation to behavioral influence in farm animals

7.1 Metabolic regulation

VSFTN plays an indispensable role in various physiological processes, prominently influencing glucose and lipid metabolism. It significantly contributes to anti-inflammatory responses, glucose and lipid modulation, and behavioral aspects related to food intake (90). In adipocytes, VSFTN-induced NAD biosynthesis acts as a crucial physiological regulator, impacting metabolic activities within AT and exerting systemic influence (91). VSFTN has a metabolic effect analogous to insulin, stimulating glucose uptake in myocytes and adipocytes, augmenting lipogenesis, and suppressing glucose release from hepatocytes (92, 93). A visual representation of these multifarious roles can be found in Figure 3.

Figure 3
www.frontiersin.org

Figure 3. Key biological roles of VSFTN: insights into lipid and glucose metabolism and inflammation.

7.2 Mechanisms

VSFTN’s influence on glucose and lipid metabolism spans endocrine, paracrine, and autocrine pathways, with its autocrine actions notably impacting insulin sensitivity in the liver (92). Research supports these findings; for instance, in a porcine cellular model, VSFTN and insulin elevated lipoprotein lipase and PPARγ mRNA expression in preadipocytes and enhanced fatty acid synthase mRNA expression in differentiated adipocytes (94). Uniquely, VSFTN also increased IL-6 mRNA expression, indicating its involvement in lipid metabolism.

7.3 Behavioral influence

VSFTN’s impact extends to behavioral modulation, particularly in regulating food intake and indirectly controlling energy balance (95). For example, an intracerebroventricular injection of VSFTN in chicks increased feed intake and altered brain activity, highlighting its role in modulating feeding behavior (96).

7.4 Dietary influence

Dietary inputs can affect VSFTN gene expression. In Hanwoo beef calves, a reduction in concentrate intake increased VSFTN gene expression in the liver, indicating diet’s pivotal role in regulating this gene (97). Furthermore, an inverse correlation between VSFTN expression and body fat levels was observed in pigs, with leaner pigs exhibiting higher VSFTN concentrations, raising questions about its reliability as an indicator of fat storage (98).

The various biological implications of VSFTN across animal studies are systematically summarized in Table 2.

Table 2
www.frontiersin.org

Table 2. Summary of findings: biological effects of VSFTN in animals.

8 Origin, molecular structure, and regulatory mechanisms of IRSN in energy homeostasis

8.1 Origin and structure

IRSN, identified as a significant myokine, is released from human muscle tissue following exercise (102). It arises from the precursor protein, fibronectin type III domain 5 (FNDC5), a type-I transmembrane protein initially described in 2002 (103, 104). Structurally, FNDC5 comprises an N-terminal peptide chain (AA sequence 1–28), a Fibronectin-III domain (AA sequence 33–124), a transmembrane domain (AA sequence 150–170), and a cytoplasmic tail (AA sequence 171–209) (105). The extracellular N-terminal tail undergoes proteolytic cleavage, releasing the 112 AA IRSN peptide that circulates across various tissues (102).

8.2 Regulatory mechanisms

FNDC5 gene expression is modulated by pivotal proteins like peroxisome proliferator-activated receptor gamma (PPARγ) and coactivator PGC1α (106). PPARγ governs adipocyte differentiation and lipid metabolism, influencing processes such as anti-inflammatory responses, lipid storage in the liver, and glucose-stimulated insulin secretion in pancreatic beta cells (107109). Conversely, PGC1α is renowned for overseeing mitochondrial biogenesis and regulating oxidative metabolism in diverse cell types (110).

8.3 Role in farm animals

Recent studies have further elucidated IRSN’s role in farm animals. One study established that delivery mode affects IRSN concentrations in Holstein calves. Dystocia and cesarean-born calves presented reduced IRSN levels post-colostrum intake, while those born vaginally showed a decline by day 15, highlighting the relationship between birth methods and metabolic adaptations via IRSN concentrations (111). Moreover, IRSN concentrations were notably heightened in cattle with subclinical ketosis compared to their healthy counterparts. This increase was accompanied by a pronounced positive correlation between IRSN and ghrelin levels, indicating IRSN’s potential as a ketosis biomarker (112). Additionally, IRSN has been shown to impact glucose metabolism in cattle by reducing mRNA levels of certain glucose transporters in granulosa cells and increasing lactate release (113).

A positive IRSN-leptin relationship, particularly in cows with subclinical ketosis, aligns with prior studies connecting insulin and IRSN in metabolic disorders (114117). These findings underscore IRSN’s multifaceted role in farm animals, linking birth methods to IRSN levels and metabolic adjustments. Its elevated concentration in ketotic cattle and associations with ghrelin and leptin further indicate IRSN’s potential as a biomarker for metabolic disorders, specifically subclinical ketosis, and its influence on glucose metabolism.

9 Species-specific expressions and uncharted territories of IRSN in farm animals

Recent studies have begun exploring the role and expression of FNDC5 and IRSN in farm animals, revealing differences from humans and mice. For instance, the bovine genome shows higher transcript variability of FNDC5 compared to humans and mice. Although FNDC5 protein distribution remains consistent in bull skeletal muscles, mRNA transcript levels vary significantly in AT and the liver (118). However, detecting IRSN in cattle plasma remains challenging (119).

Further complicating the picture, Daudon et al. (15) posited that FNDC5 and IRSN play roles in lipid mobilization in AT of dairy cattle post-calving. The emerging picture indicates varying and sometimes conflicting views on IRSN’s expression and effects in cattle, warranting deeper investigations. Beyond cattle, the exploration of IRSN’s role in other farm animals has begun. For example, IRSN, FNDC5, and PGC1α were detected in skeletal muscles and WATs of dromedary camels, with correlations observed between their levels and metabolic responses to exercise (120). Further, the IRSN peptide was localized in swine ovaries, suggesting implications for ovarian function (121). Another study on Arabian horses linked serum IRSN levels to exercise regimes (122).

While the above findings shed some light, the overarching theme is clear: Our understanding of IRSN in farm animals, especially its implications on energy regulation, remains limited. Much of the IRSN research focus has historically been on humans and lab models, like mice and rats. This current state presents an extensive opportunity to investigate IRSN’s role in farm animals more comprehensively, aligning with the broader aim of deciphering its potential implications in energy regulation within this context.

10 IRSN in metabolic regulation, energy expenditure, and implications for farm animals

10.1 Metabolic roles

IRSN is a prominent adipocytokine deeply involved in various metabolic pathways, influencing lipid homeostasis, cardiovascular health, CNS processes, and overall energy metabolism (123, 124). It plays a central role in converting WAT to BAT, thus amplifying energy expenditure (125). A detailed depiction of the signaling pathways activated by IRSN is provided in Figure 4.

Figure 4
www.frontiersin.org

Figure 4. Activation of signaling pathways triggered by IRSN expression.

IRSN stimulates glycolysis and oxidative metabolism, endorsing mitochondrial biogenesis via key genes like Glut4 and UCP3, enhancing energy output, insulin sensitivity, and a healthier metabolic profile (126). These effects are mediated through various pathways, including cAMP-PKA-HSL (126).

10.2 Liver metabolism and thermogenesis

IRSN influences liver metabolism by stimulating key pathways and enzymes such as AMPK and LKB1, improving hepatic glucose and lipid metabolism (127, 128). The upregulation of UCP1 in BAT aids thermogenesis and energy expenditure, promoting weight loss and enhancing glucose metabolism (129).

10.3 Modulation by physiological changes

Physical activity significantly affects IRSN expression, with exercise increasing its plasma and skeletal muscle levels, and extended durations enriching its presence in the brain, potentially reducing anxiety (130). IRSN levels are also modulated by dietary adjustments, obesity, and specific pharmacological exposures (16). For a comprehensive overview of how physical activity impacts the transcription of the FNDC5 gene and leads to the release of IRSN, refer to Figure 5.

Figure 5
www.frontiersin.org

Figure 5. Physical activity stimulates DNA transcription of the FNDC5 gene, leading to proteolytic cleavage and subsequent release of the IRSN.

10.4 Implications for farm animals

In farm animals, IRSN shows intriguing responses. For example, camels exhibit a relationship between glucose and IRSN during exercise, suggesting regulatory roles of glucose, FFA, insulin, leptin, and cortisol on the PGC-1α/FNDC5/IRSN pathway (120). Postpartum dairy cows show correlations between FNDC5 plasma concentrations and various metabolic metrics, emphasizing IRSN’s importance during this period (15). In dairy cattle, IRSN plays a significant role in lipid metabolism, enhancing lipolysis and mobilizing lipid reserves post-parturition (15).

IRSN’s diverse roles in metabolic regulation and energy expenditure highlight its potential in improving health and productivity in farm animals. Understanding its pathways and effects can lead to innovative strategies for managing livestock metabolism.

Table 3 elucidates the biological effects of IRSN in laboratory animals and presents an all-encompassing summary of the observed results.

Table 3
www.frontiersin.org

Table 3. Summary of findings: biological effects of IRSN in laboratory animal models.

11 Roles of APLN, VSFTN, and IRSN in metabolic adaptations in farm animals

Farm animals, notably dairy cattle, undergo significant metabolic adjustments during early lactation. These shifts correlate with milk production and an observed disparity in feed intake, frequently leading to an NEB — a situation where energy demands outstrip consumption, with critical repercussions for post-calving health (137, 138). As they transition from late pregnancy to early lactation, there’s a marked decrease in insulin plasma levels, coupled with diminished insulin sensitivity in key tissues like skeletal muscle and AT (139). These alterations ensure glucose is adequately available for milk synthesis and fetal development, while heightened insulin resistance augments lipid mobilization, leading to elevated plasma NEFA and beta-hydroxybutyrate levels post-calving (140144).

Adipokines, namely APLN, VSFTN, and IRSN, play instrumental roles in these metabolic transitions. Specifically, in dairy cows, APLN-36, a variant of APLN, exhibits elevated concentration and mRNA expression nearing parturition, showing an inverse relationship with serum NEFA levels. This suggests APLN’s potential to modulate lipid mobilization in dairy cows (51, 145, 146). VSFTN, with its critical function in insulin sensitivity and glucose regulation, gains prominence during the pregnancy-to-lactation transition, especially in high-producing dairy cows. Given its presence in mammary gland epithelial cells and milk, VSFTN might offer health benefits to calves (80, 147, 148). Conversely, IRSN is vital in lipid mobilization during post-partum NEB, with elevated plasma levels observed after calving (15).

In a study, diet-restricted calves displayed heightened VSFTN mRNA expression in liver biopsies versus controls, pointing to potential glucose metabolism irregularities and indicating the profound effect of diet on VSFTN expression and glucose regulation (97).

Furthermore, optimizing fat deposition in farm animals directly impacts meat quality. While some fats might be superfluous, intramuscular fat enhances flavor. The production of IRSN during physical activity could influence IM fat deposition, suggesting its potential to elevate meat quality (149).

The interplay between APLN, VSFTN, and IRSN in energy balance and metabolism, particularly in insulin resistance and obesity, is noteworthy. APLN levels are higher in obesity but drop with weight loss, while IRSN decreases in obesity but increases during exercise (150). Investigations have delved into the dynamics between these adipokines and metabolic parameters, revealing their fluctuating levels under normal, impaired glucose tolerance, and diabetic conditions (151). Unraveling these relationships and understanding their nuances is essential for the energy metabolism of farm animals and demands more in-depth exploration. The effects of the three adipokines on farm animals are summarized in Table 4.

Table 4
www.frontiersin.org

Table 4. Summary of biological effects of APLN, VSFTN, and IRSN in farm animals.

Overall, APLN, VSFTN, and IRSN have pivotal roles in energy regulation in farm animals, especially during crucial metabolic transitions. Enhancing our understanding of these adipokines in farm animal contexts is fundamental for refining health and production strategies.

12 Energy regulation and reproduction in farm animals: effects of APLN, VSFTN, and IRSN

Farm animal fertility is intricately linked to energy metabolism. With the hypothalamus, anterior pituitary, and gonads collectively governing the reproductive system, energy status emerges as a determinant of fertility. In recent years, AT has evolved from being perceived merely as an energy storage site to an active endocrine organ, releasing a slew of adipokines. Notably, leptin and adiponectin have been pinpointed for their involvement in the hypothalamic–pituitary-gonadal axis and female reproductive tract. Yet, the adipokines APLN, VSTFN, and IRSN have garnered attention for their potential roles within various female reproductive systems of farm animals (20).

APLN and its receptor, APJ, are discernible in the ovaries across several farm animals, ranging from cattle to sheep (43, 152155). Besides the ovaries, APLN is also detectable in sheep mammary glands (44). Furthermore, APLN has been identified in the uterus and uterine tubes as well as in the ovary (42). This adipokine has been found to augment steroidogenesis in several species, including cattle and porcine, and stimulate the proliferation of granulosa cells (152, 153, 156).

VSFTN’s presence is affirmed in the ovaries of animals like cattle, buffalo, chicken, and turkeys (89, 157159). Its functional role varies across species; while it boosts steroidogenesis and granulosa cell proliferation in cattle, buffalo, and turkeys, its effect seems inverse in chickens (89).

IRSN’s landscape in farm animals is less explored. Though observed in porcine (121), its gene expression in cattle diverges from patterns seen in humans and mice (118). Preliminary data suggest the absence of IRSN expression in buffalo ovaries. IRSN is noted to influence steroidogenesis in porcine ovaries, but its broader implications for the reproductive systems of farm animals remain enigmatic.

Despite the evidence indicating adipokine involvement in certain species, data gaps exist, especially concerning their interactions with the hypothalamus-pituitary axis in farm animals. To realize the full scope of APLN, VSFTN, and IRSN’s roles in energy regulation and reproduction, targeted research in the context of farm animals is paramount.

13 Applications of APLN, VSFTN, and IRSN in farm animal production

In ruminants, such as sheep and goats, the role of APLN extends beyond mere energy regulation. It is intricately involved in postprandial responses and profoundly affects the secretion of growth hormone, arginine-vasopressin, and adrenocorticotropic hormones (160). Specifically, in sheep, APLN’s ability to modulate molecules is evident in its regulation of mammary gland activity. This regulation is characterized by the induction of hormonal activation and a biphasic hemodynamic response (60). During different physiological stages in ewes, such as lactation and pregnancy, serum APLN levels appear to be resilient to alterations in the body condition score (BCS). This consistent presence underlines its potential importance in energy regulation during these critical phases (161). Post-parturition, decreased levels of APLN are observed, suggesting its potential adaptive role during this period (146).

Dairy cows present another dimension to the understanding of APLN. Norvezh et al. (51) highlighted a decline in serum APLN-36 levels post-calving. This fluctuation is closely associated with blood biochemical parameters, indicative of the cow’s transition to an NEB state. Such alterations in APLN levels may be instrumental in helping dairy cows accommodate the increased energy requirements characteristic of lactation. Furthermore, cow’s milk represents a key dietary component for calves and humans. Rich in various adipokines, it offers both nutritional and physiological benefits. APLN, as a part of this adipokine profile, could be crucial for growth and overall health, emphasizing the milk’s value not just as a dietary component but as a potential modulator of energy regulation (162). Other findings in sheep showed that APLN levels in ewes varied significantly based on breed, gender, and their interactions with body condition score, but not by lactation or pregnancy status (161). These authors claimed that the variability in APLN levels during critical physiological phases and its potential role as a serum biomarker strongly suggest its potential application in diagnosing and understanding metabolic disorders (161). Similarly, APLN levels in dairy cows’ serum stayed stable between pregnancy and lactation, indicating slight fluctuation (52).

With the pivotal roles that APLN, VSFTN, and IRSN play in energy regulation across farm animals, it’s evident that understanding their dynamics can offer valuable insights. These insights can potentially drive advancements in farm animal production strategies, with health, growth, and reproductive efficiency implications.

14 Future research focus

Currently, there is a significant gap in knowledge regarding the specific roles of novel adipokines—APLN, VSFTN, and IRSN—in farm animals, particularly in terms of energy metabolism and production. Limited information is available on their impact, especially concerning VSFTN. Future research should aim to investigate the associations between these adipokines and their combined effects on energy regulation. Understanding these relationships will provide valuable insights into their physiological roles and potential applications for enhancing farm animal health and productivity.

Research priorities:

1. Interplay of adipokines: Investigate how changes in one adipokine influence the levels or functions of the others.

2. Impact on energy metabolism: Study the specific roles of APLN, VSFTN, and IRSN in energy metabolism in various farm animals.

3. Production outcomes: Assess the effects of these adipokines on farm animal production metrics, such as growth, milk yield, and meat quality.

4. Mechanistic studies: Conduct detailed mechanistic studies to understand the molecular pathways mediated by these adipokines.

5. Comparative analysis: Compare the roles and effects of these adipokines in farm animals with those observed in model animals to identify species-specific differences and similarities.

Author contributions

BS: Conceptualization, Data curation, Formal analysis, Funding acquisition, Investigation, Methodology, Project administration, Resources, Software, Supervision, Validation, Visualization, Writing – original draft, Writing – review & editing. S-SJ: Writing - Review & editing HL: Writing – review & editing. HA: Writing – review & editing. AS: Writing – review & editing. AG: Writing – review & editing. SM: Writing – review & editing. SA: Writing – review & editing.

Funding

The author(s) declare that no financial support was received for the research, authorship, and/or publication of this article.

Conflict of interest

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

Publisher’s note

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

References

1. Ràfols, ME . Adipose tissue: cell heterogeneity and functional diversity. Endocrinol Nutr. (2014) 61:100–12. doi: 10.1016/j.endonu.2013.03.011

PubMed Abstract | Crossref Full Text | Google Scholar

2. Sauerwein, H, Bendixen, E, Restelli, L, and Ceciliani, F. The adipose tissue in farm animals: a proteomic approach. Curr Protein Pept Sci. (2014) 15:146–55. doi: 10.2174/1389203715666140221123105

PubMed Abstract | Crossref Full Text | Google Scholar

3. Chernukha, IM, Fedulova, LV, and Kotenkova, EA. White, beige and brown adipose tissue: structure, function, specific features and possibility formation and divergence in pigs. Foods Raw Mater. (2022) 10:10–8. doi: 10.21603/2308-4057-2022-1-10-18

Crossref Full Text | Google Scholar

4. Fain, JN, Madan, AK, Hiler, ML, Cheema, P, and Bahouth, SW. Comparison of the release of adipokines by adipose tissue, adipose tissue matrix, and adipocytes from visceral and subcutaneous abdominal adipose tissues of obese humans. Endocrinology. (2004) 145:2273–82. doi: 10.1210/en.2003-1336

PubMed Abstract | Crossref Full Text | Google Scholar

5. Lee, JH, Park, A, Oh, K-J, Lee, SC, Kim, WK, and Bae, K-H. The role of adipose tissue mitochondria: regulation of mitochondrial function for the treatment of metabolic diseases. Int J Mol Sci. (2019) 20:4924. doi: 10.3390/ijms20194924

PubMed Abstract | Crossref Full Text | Google Scholar

6. Radin, MJ, Sharkey, LC, and Holycross, BJ. Adipokines: a review of biological and analytical principles and an update in dogs, cats, and horses. Vet Clin Pathol. (2009) 38:136–56. doi: 10.1111/j.1939-165X.2009.00133.x

Crossref Full Text | Google Scholar

7. Raucci, R, Rusolo, F, Sharma, A, Colonna, G, Castello, G, and Costantini, S. Functional and structural features of adipokine family. Cytokine. (2013) 61:1–14. doi: 10.1016/j.cyto.2012.08.036

PubMed Abstract | Crossref Full Text | Google Scholar

8. Palin, M-F, Farmer, C, and Duarte, C. Triennial lactation symposium/bolfa: Adipokines affect mammary growth and function in farm animals. J Anim Sci. (2017) 95:5689–700. doi: 10.2527/jas2017.1777

PubMed Abstract | Crossref Full Text | Google Scholar

9. O’Carroll, A-M, Lolait, SJ, Harris, LE, and Pope, GR. The apelin receptor APJ: journey from an orphan to a multifaceted regulator of homeostasis. J Endocrinol. (2013) 219:R13–35. doi: 10.1530/JOE-13-0227

PubMed Abstract | Crossref Full Text | Google Scholar

10. Castan-Laurell, I, Vítkova, M, Daviaud, D, Dray, C, Kováčiková, M, Kovacova, Z, et al. Effect of hypocaloric diet-induced weight loss in obese women on plasma apelin and adipose tissue expression of apelin and APJ. Eur J Endocrinol. (2008) 158:905–10. doi: 10.1530/EJE-08-0039

PubMed Abstract | Crossref Full Text | Google Scholar

11. Dray, C, Knauf, C, Daviaud, D, Waget, A, Boucher, J, Buleon, M, et al. Apelin stimulates glucose utilization in normal and obese insulin-resistant mice. Cell Metab. (2008) 8:437–45. doi: 10.1016/j.cmet.2008.10.003

PubMed Abstract | Crossref Full Text | Google Scholar

12. Kaczor, U, Jurkowska, M, Kucharski, M, and Kaczor, A. Protein function and polymorphism of the Visfatin gene in farm animals. Rocz Nauk Zoot. (2017) 44:133–9.

Google Scholar

13. Chen, H, Xia, T, Zhou, L, Chen, X, Gan, L, Yao, W, et al. Gene organization, alternate splicing and expression pattern of porcine visfatin gene. Domest Anim Endocrinol. (2007) 32:235–45. doi: 10.1016/j.domaniend.2006.03.004

Crossref Full Text | Google Scholar

14. Tond, SB, Fallah, S, Salemi, Z, and Seifi, M. Influence of mulberry leaf extract on serum adiponectin, visfatin and lipid profile levels in type 2 diabetic rats. Braz Arch Biol Technol. (2016) 59:59. doi: 10.1590/1678-4324-2016160297

Crossref Full Text | Google Scholar

15. Daudon, M, Bigot, Y, Dupont, J, and Price, CA. Irisin and the fibronectin type III domain-containing family: structure, signaling and role in female reproduction. Reproduction. (2022) 164:R1–9. doi: 10.1530/REP-22-0037

PubMed Abstract | Crossref Full Text | Google Scholar

16. Mahgoub, MO, D’Souza, C, Al Darmaki, RS, Baniyas, MM, and Adeghate, E. An update on the role of irisin in the regulation of endocrine and metabolic functions. Peptides. (2018) 104:15–23. doi: 10.1016/j.peptides.2018.03.018

PubMed Abstract | Crossref Full Text | Google Scholar

17. Arhire, LI, Mihalache, L, and Covasa, M. Irisin: a hope in understanding and managing obesity and metabolic syndrome. Front Endocrinol. (2019) 10:524. doi: 10.3389/fendo.2019.00524

PubMed Abstract | Crossref Full Text | Google Scholar

18. Polyzos, SA, Kountouras, J, Shields, K, and Mantzoros, CS. Irisin: a renaissance in metabolism? Metabolism. (2013) 62:1037–44. doi: 10.1016/j.metabol.2013.04.008

PubMed Abstract | Crossref Full Text | Google Scholar

19. Block, S, Butler, W, Ehrhardt, R, Bell, A, Van Amburgh, M, and Boisclair, Y. Decreased concentration of plasma leptin in periparturient dairy cows is caused by negative energy balance. J Endocrinol. (2001) 171:339–48. doi: 10.1677/joe.0.1710339

PubMed Abstract | Crossref Full Text | Google Scholar

20. Shokrollahi, B, Shang, JH, Saadati, N, Ahmad, HI, and Yang, CY. Reproductive roles of novel adipokines apelin, visfatin, and irisin in farm animals. Theriogenology. (2021) 172:178–86. doi: 10.1016/j.theriogenology.2021.06.011

PubMed Abstract | Crossref Full Text | Google Scholar

21. Tatemoto, K, Hosoya, M, Habata, Y, Fujii, R, Kakegawa, T, Zou, M-X, et al. Isolation and characterization of a novel endogenous peptide ligand for the human APJ receptor. Biochem Biophys Res Commun. (1998) 251:471–6. doi: 10.1006/bbrc.1998.9489

PubMed Abstract | Crossref Full Text | Google Scholar

22. Coquerel, D, Delile, E, Dumont, L, Chagnon, F, Murza, A, Sainsily, X, et al. Gαi-biased apelin analog protects against isoproterenol-induced myocardial dysfunction in rats. Am J Physiol Heart Circ Physiol. (2021) 320:H1646–56. doi: 10.1152/ajpheart.00688.2020

PubMed Abstract | Crossref Full Text | Google Scholar

23. Shin, K, Chapman, NA, Sarker, M, Kenward, C, Huang, SK, Weatherbee-Martin, N, et al. Bioactivity of the putative apelin proprotein expands the repertoire of apelin receptor ligands. Biochim Biophys Acta Gen Subj. (2017) 1861:1901–12. doi: 10.1016/j.bbagen.2017.05.017

PubMed Abstract | Crossref Full Text | Google Scholar

24. Shin, K, Kenward, C, and Rainey, JK. Apelinergic system structure and function. Compr Physiol. (2017) 8:407–50. doi: 10.1002/cphy.c170028

PubMed Abstract | Crossref Full Text | Google Scholar

25. Ma, Y, Yue, Y, Ma, Y, Zhang, Q, Zhou, Q, Song, Y, et al. Structural basis for apelin control of the human apelin receptor. Structure. (2017) 25:858–866.e4. doi: 10.1016/j.str.2017.04.008

PubMed Abstract | Crossref Full Text | Google Scholar

26. Langelaan, DN, Bebbington, EM, Reddy, T, and Rainey, JK. Structural insight into G-protein coupled receptor binding by apelin. Biochemistry. (2009) 48:537–48. doi: 10.1021/bi801864b

PubMed Abstract | Crossref Full Text | Google Scholar

27. Zhen, EY, Higgs, RE, and Gutierrez, JA. Pyroglutamyl apelin-13 identified as the major apelin isoform in human plasma. Anal Biochem. (2013) 442:1–9. doi: 10.1016/j.ab.2013.07.006

Crossref Full Text | Google Scholar

28. Kurowska, P, Barbe, A, Różycka, M, Chmielińska, J, Dupont, J, and Rak, A. Apelin in reproductive physiology and pathology of different species: a critical review. Int J Endocrinol. (2018) 2018:1–12. doi: 10.1155/2018/9170480

Crossref Full Text | Google Scholar

29. Wang, G, Qi, X, Wei, W, Englander, EW, and Greeley, GH Jr. Characterization of the 5′-regulatory regions of the rat and human apelin genes and regulation of breast apelin by USF. FASEB J. (2006) 20:2639–41. doi: 10.1096/fj.06-6315fje

PubMed Abstract | Crossref Full Text | Google Scholar

30. Salska, A, and Chiżyński, K. Apelin–a potential target in the diagnosis and treatment of the diseases of civilization. Acta Cardiol. (2016) 71:505–17. doi: 10.1080/AC.71.5.3167493

Crossref Full Text | Google Scholar

31. Gandham, R, Sumathi, M, Dayanand, C, Sheela, S, and Kiranmayee, P. Apelin and its receptor: an overview. J Clin Diagn Res. (2019) 13:EE01–5. doi: 10.7860/JCDR/2019/41074.12930

Crossref Full Text | Google Scholar

32. Lee, DK, Cheng, R, Nguyen, T, Fan, T, Kariyawasam, AP, Liu, Y, et al. Characterization of apelin, the ligand for the APJ receptor. J Neurochem. (2000) 74:34–41. doi: 10.1046/j.1471-4159.2000.0740034.x

Crossref Full Text | Google Scholar

33. Langelaan, DN. Structural studies of apelin and its receptor as well as the characteristics and causes of membrane protein helix kinks (Master’s thesis). Dalhousie University. (2013).

Google Scholar

34. Wei, L, Hou, X, and Tatemoto, K. Regulation of apelin mRNA expression by insulin and glucocorticoids in mouse 3T3-L1 adipocytes. Regul Pept. (2005) 132:27–32. doi: 10.1016/j.regpep.2005.08.003

PubMed Abstract | Crossref Full Text | Google Scholar

35. Lv, S-Y, Cui, B, Chen, W-D, and Wang, Y-D. Apelin/APJ system: a key therapeutic target for liver disease. Oncotarget. (2017) 8:112145:–112151. doi: 10.18632/oncotarget.22841

PubMed Abstract | Crossref Full Text | Google Scholar

36. Hu, G, Wang, Z, Zhang, R, Sun, W, and Chen, X. The role of Apelin/Apelin receptor in energy metabolism and water homeostasis: a comprehensive narrative review. Front Physiol. (2021) 12:632886. doi: 10.3389/fphys.2021.632886

PubMed Abstract | Crossref Full Text | Google Scholar

37. Pope, GR, Roberts, EM, Lolait, SJ, and O’Carroll, A-M. Central and peripheral apelin receptor distribution in the mouse: species differences with rat. Peptides. (2012) 33:139–48. doi: 10.1016/j.peptides.2011.12.005

PubMed Abstract | Crossref Full Text | Google Scholar

38. Dawid, M, Mlyczyńska, E, Jurek, M, Respekta, N, Pich, K, Kurowska, P, et al. Apelin, APJ, and ELABELA: role in placental function, pregnancy, and foetal development—an overview. Cells. (2021) 11:99. doi: 10.3390/cells11010099

PubMed Abstract | Crossref Full Text | Google Scholar

39. Volkoff, H, and Wyatt, JL. Apelin in goldfish (Carassius auratus): cloning, distribution and role in appetite regulation. Peptides. (2009) 30:1434–40. doi: 10.1016/j.peptides.2009.04.020

PubMed Abstract | Crossref Full Text | Google Scholar

40. Lin, F, Wu, H, Chen, H, Xin, Z, Yuan, D, Wang, T, et al. Molecular and physiological evidences for the role in appetite regulation of apelin and its receptor APJ in Ya-fish (Schizothorax prenanti). Mol Cell Endocrinol. (2014) 396:46–57. doi: 10.1016/j.mce.2014.08.009

PubMed Abstract | Crossref Full Text | Google Scholar

41. Hayes, J, and Volkoff, H. Characterization of the endocrine, digestive and morphological adjustments of the intestine in response to food deprivation and torpor in cunner, Tautogolabrus adspersus. Comp Biochem Physiol Part A Mol Integr Physiol. (2014) 170:46–59. doi: 10.1016/j.cbpa.2014.01.014

PubMed Abstract | Crossref Full Text | Google Scholar

42. Palmioli, E, Dall’Aglio, C, Bellesi, M, Tardella, FM, Moscatelli, S, Scocco, P, et al. The apelinergic system immuno-detection in the abomasum and duodenum of sheep grazing on semi-natural pasture. Animals. (2021) 11:173. doi: 10.3390/ani11113173

PubMed Abstract | Crossref Full Text | Google Scholar

43. Mercati, F, Scocco, P, Maranesi, M, Acuti, G, Petrucci, L, Cocci, P, et al. Apelin system detection in the reproductive apparatus of ewes grazing on semi-natural pasture. Theriogenology. (2019) 139:156–66. doi: 10.1016/j.theriogenology.2019.08.012

PubMed Abstract | Crossref Full Text | Google Scholar

44. Mercati, F, Maranesi, M, Dall Aglio, C, Petrucci, L, Pasquariello, R, Tardella, FM, et al. Apelin system in mammary gland of sheep reared in semi-natural pastures of the central apennines. Animals. (2018) 8:223. doi: 10.3390/ani8120223

Crossref Full Text | Google Scholar

45. Chang, TK, Zhong, YH, Liu, SC, Huang, CC, Tsai, CH, Lee, HP, et al. Apelin promotes endothelial progenitor cell angiogenesis in rheumatoid arthritis disease via the miR-525-5p/angiopoietin-1 pathway. Front Immunol. (2021) 12:737990. doi: 10.3389/fimmu.2021.737990

PubMed Abstract | Crossref Full Text | Google Scholar

46. Knauf, C, Drougard, A, Fournel, A, Duparc, T, and Valet, P. Hypothalamic actions of apelin on energy metabolism: new insight on glucose homeostasis and metabolic disorders. Horm Metab Res. (2013) 45:928–34. doi: 10.1055/s-0033-1351321

PubMed Abstract | Crossref Full Text | Google Scholar

47. Banerjee, A, and Singh, J. Remodeling adipose tissue inflammasome for type 2 diabetes mellitus treatment: current perspective and translational strategies. Bioeng Transl Med. (2020) 5:e10150. doi: 10.1002/btm2.10150

PubMed Abstract | Crossref Full Text | Google Scholar

48. Bertrand, C, Valet, P, and Castan-Laurell, I. Apelin and energy metabolism. Front Physiol. (2015) 6:115. doi: 10.3389/fphys.2015.00115

Crossref Full Text | Google Scholar

49. Afshounpour, MT, Habibi, A, and Ranjbar, R. Impact of combined exercise training on plasma concentration of Apelin, resistin and insulin resistance in patients with type 2 diabetics’ male. Hormozgan Med J. (2016) 20:158–69.

Google Scholar

50. Ceranowicz, P, Warzecha, Z, and Dembinski, A. Peptidyl hormones of endocrine cells origin in the gut—their discovery and physiological relevance. J Physiol Pharmacol. (2015) 66:11–27. doi: 10.26402/jpp.2015.1.01

PubMed Abstract | Crossref Full Text | Google Scholar

51. Norvezh, F, Jalali, MR, Tabandeh, MR, Hajikolaei, MRH, and Gooraninejad, S. Serum Apelin-36 alteration in late pregnancy and early lactation of dairy cows and its association with negative energy balance markers. Res Vet Sci. (2019) 125:285–9. doi: 10.1016/j.rvsc.2019.07.012

PubMed Abstract | Crossref Full Text | Google Scholar

52. Weber, M, Locher, L, Huber, K, Kenéz, Á, Rehage, J, Tienken, R, et al. Longitudinal changes in adipose tissue of dairy cows from late pregnancy to lactation. Part 1: the adipokines apelin and resistin and their relationship to receptors linked with lipolysis. J Dairy Sci. (2016) 99:1549–59. doi: 10.3168/jds.2015-10131

PubMed Abstract | Crossref Full Text | Google Scholar

53. Nadal, A, Quesada, I, Tuduri, E, Nogueiras, R, and Alonso-Magdalena, P. Endocrine-disrupting chemicals and the regulation of energy balance. Nat Rev Endocrinol. (2017) 13:536–46. doi: 10.1038/nrendo.2017.51

PubMed Abstract | Crossref Full Text | Google Scholar

54. Than, A, Cheng, Y, Foh, L-C, Leow, MK-S, Lim, SC, Chuah, YJ, et al. Apelin inhibits adipogenesis and lipolysis through distinct molecular pathways. Mol Cell Endocrinol. (2012) 362:227–41. doi: 10.1016/j.mce.2012.07.002

PubMed Abstract | Crossref Full Text | Google Scholar

55. Yue, P, Jin, H, Xu, S, Aillaud, M, Deng, AC, Azuma, J, et al. Apelin decreases lipolysis via Gq, Gi, and AMPK-dependent mechanisms. Endocrinology. (2011) 152:59–68. doi: 10.1210/en.2010-0576

PubMed Abstract | Crossref Full Text | Google Scholar

56. Xu, S, Tsao, PS, and Yue, P. Apelin and insulin resistance: another arrow for the quiver? J Diabetes. (2011) 3:225–31. doi: 10.1111/j.1753-0407.2011.00132.x

PubMed Abstract | Crossref Full Text | Google Scholar

57. Guo, R, Rogers, O, and Nair, S. Targeting Apelinergic system in Cardiometabolic disease. Curr Drug Targets. (2016) 17:1–7.

Google Scholar

58. Girault-Sotias, P-E, Gerbier, R, Flahault, A, de Mota, N, and Llorens-Cortes, C. Apelin and vasopressin: the yin and yang of water balance. Front Endocrinol. (2021) 12:735515. doi: 10.3389/fendo.2021.735515

PubMed Abstract | Crossref Full Text | Google Scholar

59. Reaux-Le Goazigo, A, Bodineau, L, De Mota, N, Jeandel, L, Chartrel, N, Knauf, C, et al. Apelin and the proopiomelanocortin system: a new regulatory pathway of hypothalamic α-MSH release. Am J Physiol Endocrinol Metab. (2011) 301:E955–66. doi: 10.1152/ajpendo.00090.2011

PubMed Abstract | Crossref Full Text | Google Scholar

60. Charles, CJ, Rademaker, MT, and Richards, AM. Apelin-13 induces a biphasic haemodynamic response and hormonal activation in normal conscious sheep. J Endocrinol. (2006) 189:701–10. doi: 10.1677/joe.1.06804

PubMed Abstract | Crossref Full Text | Google Scholar

61. Ohno, S, Yakabi, K, Ro, S, Ochiai, M, Onouchi, T, Sakurada, T, et al. Apelin-12 stimulates acid secretion through an increase of histamine release in rat stomachs. Reg Peptides. (2012) 174:71–8. doi: 10.1016/j.regpep.2011.12.002

PubMed Abstract | Crossref Full Text | Google Scholar

62. Lv, S-Y, Yang, Y-J, Qin, Y-J, Xiong, W, and Chen, Q. Effect of centrally administered apelin-13 on gastric emptying and gastrointestinal transit in mice. Peptides. (2011) 32:978–82. doi: 10.1016/j.peptides.2011.01.023

PubMed Abstract | Crossref Full Text | Google Scholar

63. Sunter, D, Hewson, AK, and Dickson, SL. Intracerebroventricular injection of apelin-13 reduces food intake in the rat. Neurosci Lett. (2003) 353:1–4. doi: 10.1016/S0304-3940(03)00351-3

PubMed Abstract | Crossref Full Text | Google Scholar

64. Frier, BC, Williams, DB, and Wright, DC. The effects of apelin treatment on skeletal muscle mitochondrial content. Am J Physiol Regul Integr Comp Physiol. (2009) 297:R1761–8. doi: 10.1152/ajpregu.00422.2009

PubMed Abstract | Crossref Full Text | Google Scholar

65. Gao, Z, Zhong, X, Tan, Y-X, and Liu, D. Apelin-13 alleviates diabetic nephropathy by enhancing nitric oxide production and suppressing kidney tissue fibrosis. Int J Mol Med. (2021) 48:1–9. doi: 10.3892/ijmm.2021.5008

Crossref Full Text | Google Scholar

66. Clarke, K, Whitaker, K, and Reyes, T. Diminished metabolic responses to centrally-administered apelin-13 in diet-induced obese rats fed a high-fat diet. J Neuroendocrinol. (2009) 21:83–9. doi: 10.1111/j.1365-2826.2008.01815.x

PubMed Abstract | Crossref Full Text | Google Scholar

67. Xu, S, Han, P, Huang, M, Wu, JC, Chang, C, Tsao, PS, et al. In vivo, ex vivo, and in vitro studies on apelin's effect on myocardial glucose uptake. Peptides. (2012) 37:320–6. doi: 10.1016/j.peptides.2012.08.004

PubMed Abstract | Crossref Full Text | Google Scholar

68. Fournel, A, Drougard, A, Duparc, T, Marlin, A, Brierley, SM, Castro, J, et al. Apelin targets gut contraction to control glucose metabolism via the brain. Gut. (2017) 66:258–69. doi: 10.1136/gutjnl-2015-310230

PubMed Abstract | Crossref Full Text | Google Scholar

69. Than, A, He, HL, Chua, SH, Xu, D, Sun, L, Leow, MK-S, et al. Apelin enhances brown adipogenesis and browning of white adipocytes. J Biol Chem. (2015) 290:14679–91. doi: 10.1074/jbc.M115.643817

PubMed Abstract | Crossref Full Text | Google Scholar

70. Liu, Q, Jiang, J, Shi, Y, Mo, Z, and Li, M. Apelin/Apelin receptor: a new therapeutic target in polycystic ovary syndrome. Life Sci. (2020) 260:118310. doi: 10.1016/j.lfs.2020.118310

PubMed Abstract | Crossref Full Text | Google Scholar

71. Nyimanu, D, Kuc, RE, Williams, TL, Bednarek, M, Ambery, P, Jermutus, L, et al. Apelin-36-[L28A] and Apelin-36-[L28C (30kDa-PEG)] peptides that improve diet induced obesity are G protein biased ligands at the apelin receptor. Peptides. (2019) 121:170139. doi: 10.1016/j.peptides.2019.170139

PubMed Abstract | Crossref Full Text | Google Scholar

72. Attané, C, Daviaud, D, Dray, C, Dusaulcy, R, Masseboeuf, M, Prévot, D, et al. Apelin stimulates glucose uptake but not lipolysis in human adipose tissue ex vivo. J Mol Endocrinol. (2011) 46:21–8. doi: 10.1677/JME-10-0105

Crossref Full Text | Google Scholar

73. Zhu, S, Sun, F, Li, W, Cao, Y, Wang, C, Wang, Y, et al. Apelin stimulates glucose uptake through the PI3K/Akt pathway and improves insulin resistance in 3T3-L1 adipocytes. Mol Cell Biochem. (2011) 353:305–13. doi: 10.1007/s11010-011-0799-0

PubMed Abstract | Crossref Full Text | Google Scholar

74. Mughal, A, Sun, C, and O’Rourke, ST. Apelin reduces nitric oxide-induced relaxation of cerebral arteries by inhibiting activation of large conductance, calcium-activated K channels. J Cardiovasc Pharmacol. (2018) 71:223–32. doi: 10.1097/FJC.0000000000000563

PubMed Abstract | Crossref Full Text | Google Scholar

75. Respekta, N, Pich, K, Dawid, M, Mlyczyńska, E, Kurowska, P, and Rak, A. The Apelinergic system: Apelin, ELABELA, and APJ action on cell apoptosis: anti-apoptotic or pro-apoptotic effect? Cells. (2022) 12:150. doi: 10.3390/cells12010150

PubMed Abstract | Crossref Full Text | Google Scholar

76. Penney, CC, and Volkoff, H. Peripheral injections of cholecystokinin, apelin, ghrelin and orexin in cavefish (Astyanax fasciatus mexicanus): effects on feeding and on the brain expression levels of tyrosine hydroxylase, mechanistic target of rapamycin and appetite-related hormones. Gen Comp Endocrinol. (2014) 196:34–40. doi: 10.1016/j.ygcen.2013.11.015

PubMed Abstract | Crossref Full Text | Google Scholar

77. Yan, X, Qin, C, Yang, G, Deng, D, Yang, L, Feng, J, et al. The regulatory role of apelin on the appetite and growth of common carp (Cyprinus carpio L.). Animals. (2020) 10:163. doi: 10.3390/ani10112163

Crossref Full Text | Google Scholar

78. Maresca, F, Palma, VD, Bevilacqua, M, Uccello, G, Taglialatela, V, Giaquinto, A, et al. Adipokines, vascular wall, and cardiovascular disease: a focused overview of the role of adipokines in the pathophysiology of cardiovascular disease. Angiology. (2015) 66:8–24. doi: 10.1177/0003319713520463

PubMed Abstract | Crossref Full Text | Google Scholar

79. Karnuah, AB, Uenishi, H, Kiuchi, S, Kojima, M, Onishi, A, Yasue, H, et al. Assignment of 64 genes expressed in 28-day-old pig embryo to radiation hybrid map. Mamm Genome. (2001) 12:518–23. doi: 10.1007/s003350020035

PubMed Abstract | Crossref Full Text | Google Scholar

80. Yonezawa, T, Haga, S, Kobayashi, Y, Takahashi, T, and Obara, Y. Visfatin is present in bovine mammary epithelial cells, lactating mammary gland and milk, and its expression is regulated by cAMP pathway. FEBS Lett. (2006) 580:6635–43. doi: 10.1016/j.febslet.2006.11.014

PubMed Abstract | Crossref Full Text | Google Scholar

81. Dahl, TB, Holm, S, Aukrust, P, and Halvorsen, B. Visfatin/NAMPT: a multifaceted molecule with diverse roles in physiology and pathophysiology. Annu Rev Nutr. (2012) 32:229–43. doi: 10.1146/annurev-nutr-071811-150746

PubMed Abstract | Crossref Full Text | Google Scholar

82. Butler, MJ, and Volkoff, H. The role of visfatin/NAMPT in the regulation of feeding in goldfish (Carassius auratus). Peptides. (2023) 160:170919. doi: 10.1016/j.peptides.2022.170919

PubMed Abstract | Crossref Full Text | Google Scholar

83. Garten, A, Schuster, S, Penke, M, Gorski, T, De Giorgis, T, and Kiess, W. Physiological and pathophysiological roles of NAMPT and NAD metabolism. Nat Rev Endocrinol. (2015) 11:535–46. doi: 10.1038/nrendo.2015.117

PubMed Abstract | Crossref Full Text | Google Scholar

84. Romacho, T, Elsen, M, Röhrborn, D, and Eckel, J. Adipose tissue and its role in organ crosstalk. Acta Physiol. (2014) 210:733–53. doi: 10.1111/apha.12246

Crossref Full Text | Google Scholar

85. Revollo, JR, Körner, A, Mills, KF, Satoh, A, Wang, T, Garten, A, et al. Nampt/PBEF/visfatin regulates insulin secretion in β cells as a systemic NAD biosynthetic enzyme. Cell Metab. (2007) 6:363–75. doi: 10.1016/j.cmet.2007.09.003

PubMed Abstract | Crossref Full Text | Google Scholar

86. Revollo, JR, Grimm, AA, and Imai, S. The regulation of nicotinamide adenine dinucleotide biosynthesis by Nampt/PBEF/visfatin in mammals. Curr Opin Gastroenterol. (2007) 23:164–70. doi: 10.1097/MOG.0b013e32801b3c8f

PubMed Abstract | Crossref Full Text | Google Scholar

87. Costford, SR, Bajpeyi, S, Pasarica, M, Albarado, DC, Thomas, SC, Xie, H, et al. Skeletal muscle NAMPT is induced by exercise in humans. Am J Physiol Endocrinol Metab. (2010) 298:E117–26. doi: 10.1152/ajpendo.00318.2009

PubMed Abstract | Crossref Full Text | Google Scholar

88. Maillard, V, Elis, S, Desmarchais, A, Hivelin, C, Lardic, L, Lomet, D, et al. Visfatin and resistin in gonadotroph cells: expression, regulation of LH secretion and signalling pathways. Reprod Fertil Dev. (2017) 29:2479–95. doi: 10.1071/RD16301

PubMed Abstract | Crossref Full Text | Google Scholar

89. Ons, E, Gertler, A, Buyse, J, Lebihan-Duval, E, Bordas, A, Goddeeris, B, et al. Visfatin gene expression in chickens is sex and tissue dependent. Domest Anim Endocrinol. (2010) 38:63–74. doi: 10.1016/j.domaniend.2009.08.007

PubMed Abstract | Crossref Full Text | Google Scholar

90. Zhang, Y, Huo, Y, He, W, Liu, S, Li, H, and Li, L. Visfatin is regulated by interleukin 6 and affected by the PPAR γ pathway in BeWo cells. Mol Med Rep. (2019) 19:400–6. doi: 10.3892/mmr.2018.9671

PubMed Abstract | Crossref Full Text | Google Scholar

91. Stromsdorfer, KL, Yamaguchi, S, Yoon, MJ, Moseley, AC, Franczyk, MP, Kelly, SC, et al. NAMPT-mediated NAD+ biosynthesis in adipocytes regulates adipose tissue function and multi-organ insulin sensitivity in mice. Cell Rep. (2016) 16:1851–60. doi: 10.1016/j.celrep.2016.07.027

PubMed Abstract | Crossref Full Text | Google Scholar

92. Saddi-Rosa, P, Oliveira, CS, Giuffrida, F, and Reis, AF. Visfatin, glucose metabolism and vascular disease: a review of evidence. Diabetol Metab Syndr. (2010) 2:1–6. doi: 10.1186/1758-5996-2-21

Crossref Full Text | Google Scholar

93. Mayi, TH, Duhem, C, Copin, C, Bouhlel, MA, Rigamonti, E, Pattou, F, et al. Visfatin is induced by peroxisome proliferator-activated receptor gamma in human macrophages. FEBS J. (2010) 277:3308–20. doi: 10.1111/j.1742-4658.2010.07729.x

PubMed Abstract | Crossref Full Text | Google Scholar

94. Yang, C, Deng, S, Hsu, C, Liu, B, Lin, E, Cheng, W, et al. Visfatin regulates genes related to lipid metabolism in porcine adipocytes. J Anim Sci. (2010) 88:3233–41. doi: 10.2527/jas.2010-2799

PubMed Abstract | Crossref Full Text | Google Scholar

95. Pourvali-Talatappeh, P, and Alipoor, E. Visfatin; a potential novel mediator of brown adipose tissue. Obes Med. (2019) 15:100122. doi: 10.1016/j.obmed.2019.100122

Crossref Full Text | Google Scholar

96. Cline, MA, Nandar, W, Prall, BC, Bowden, CN, and Denbow, DM. Central visfatin causes orexigenic effects in chicks. Behav Brain Res. (2008) 186:293–7. doi: 10.1016/j.bbr.2007.08.016

PubMed Abstract | Crossref Full Text | Google Scholar

97. Chang, S, Lohakare, J, Singh, N, Kwon, E, Nejad, J, Sung, K, et al. Limiting concentrate during growing period affect performance and gene expression of hepatic gluconeogenic enzymes and visfatin in Korean native beef calves. Asian Australas J Anim Sci. (2013) 26:202–10. doi: 10.5713/ajas.2012.12442

PubMed Abstract | Crossref Full Text | Google Scholar

98. Palin, M-F, Labrecque, B, Beaudry, D, Mayhue, M, Bordignon, V, and Murphy, BD. Visfatin expression is not associated with adipose tissue abundance in the porcine model. Domest Anim Endocrinol. (2008) 35:58–73. doi: 10.1016/j.domaniend.2008.01.008

Crossref Full Text | Google Scholar

99. Sun, Q, Li, L, Li, R, Yang, M, Liu, H, Nowicki, MJ, et al. Overexpression of visfatin/PBEF/Nampt alters whole-body insulin sensitivity and lipid profile in rats. Annal Med. (2009) 41:311–20. doi: 10.1080/07853890902729760

PubMed Abstract | Crossref Full Text | Google Scholar

100. Kang, YS, Lee, MH, Song, HK, Kim, JE, Ghee, JY, Cha, JJ, et al. Chronic administration of visfatin ameliorated diabetic nephropathy in type 2 diabetic mice. Kidney Blood Pres Res. (2016) 41:311–24. doi: 10.1159/000443433

PubMed Abstract | Crossref Full Text | Google Scholar

101. Li, Z, Liu, X, Zhang, P, Han, R, Sun, G, Jiang, R, et al. Comparative transcriptome analysis of hypothalamus-regulated feed intake induced by exogenous visfatin in chicks. BMC Genomics. (2018) 19:1–17. doi: 10.1186/s12864-018-4644-7

Crossref Full Text | Google Scholar

102. Bostrom, P, Wu, J, Jedrychowski, MP, Korde, A, Ye, L, Lo, JC, et al. A PGC1-alpha-dependent myokine that drives brown-fat-like development of white fat and thermogenesis. Nature. (2012) 481:463–8. doi: 10.1038/nature10777

PubMed Abstract | Crossref Full Text | Google Scholar

103. Ferrer-Martinez, A, Ruiz-Lozano, P, and Chien, KR. Mouse PeP: a novel peroxisomal protein linked to myoblast differentiation and development. Dev Dyn. (2002) 224:154–67. doi: 10.1002/dvdy.10099

PubMed Abstract | Crossref Full Text | Google Scholar

104. Teufel, A, Malik, N, Mukhopadhyay, M, and Westphal, H. Frcp1 and Frcp2, two novel fibronectin type III repeat containing genes. Gene. (2002) 297:79–83. doi: 10.1016/S0378-1119(02)00828-4

PubMed Abstract | Crossref Full Text | Google Scholar

105. Jodeiri Farshbaf, M, and Alviña, K. Multiple roles in neuroprotection for the exercise derived myokine irisin. Front Aging Neurosci. (2021) 13:649929. doi: 10.3389/fnagi.2021.649929

PubMed Abstract | Crossref Full Text | Google Scholar

106. Jamwal, S, Blackburn, JK, and Elsworth, JD. PPARγ/PGC1α signaling as a potential therapeutic target for mitochondrial biogenesis in neurodegenerative disorders. Pharmacol Ther. (2021) 219:107705. doi: 10.1016/j.pharmthera.2020.107705

PubMed Abstract | Crossref Full Text | Google Scholar

107. Ahmadian, M, Suh, JM, Hah, N, Liddle, C, Atkins, AR, Downes, M, et al. PPARγ signaling and metabolism: the good, the bad and the future. Nat Med. (2013) 19:557–66. doi: 10.1038/nm.3159

PubMed Abstract | Crossref Full Text | Google Scholar

108. Han, L, Shen, W-J, Bittner, S, Kraemer, FB, and Azhar, S. PPARs: regulators of metabolism and as therapeutic targets in cardiovascular disease. Part II: PPAR-β/δ and PPAR-γ. Futur Cardiol. (2017) 13:279–96. doi: 10.2217/fca-2017-0019

PubMed Abstract | Crossref Full Text | Google Scholar

109. Hong, F, Pan, S, Guo, Y, Xu, P, and Zhai, Y. PPARs as nuclear receptors for nutrient and energy metabolism. Molecules. (2019) 24:2545. doi: 10.3390/molecules24142545

PubMed Abstract | Crossref Full Text | Google Scholar

110. Dabrowska, A, Venero, JL, Iwasawa, R, Hankir, M-k, Rahman, S, Boobis, A, et al. PGC-1α controls mitochondrial biogenesis and dynamics in lead-induced neurotoxicity. Aging (Albany NY). (2015) 7:629–43. doi: 10.18632/aging.100790

Crossref Full Text | Google Scholar

111. Kızıl, M, Rişvanli, A, Abay, M, Şafak, T, Kılınç, MA, Yılmaz, Ö, et al. Effect of calf delivery mode on İrisin, Asprosin, leptin, adiponectin, and İnsulin-like growth Factor-1 levels in dairy cattle and their calves. Turk J Vet Anim Sci. (2022) 55:1527. doi: 10.17582/journal.pjz/20221031081040

Crossref Full Text | Google Scholar

112. Eğritağ, HE, Merhan, O, Bozukluhan, K, Varol, K, and Atcali, T. Investigation of serum leptin, ghrelin, irisin, insulin levels and their correlations in cattle with subclinical ketosis. Vet J Mehmet Akif Ersoy Univ. (2022) 7:223–8. doi: 10.24880/maeuvfd.1202455

Crossref Full Text | Google Scholar

113. Daudon, M, Ramé, C, Price, C, and Dupont, J. Irisin modulates glucose metabolism and inhibits steroidogenesis in bovine granulosa cells. Reproduction. (2023) 165:533–42. doi: 10.1530/REP-22-0404

PubMed Abstract | Crossref Full Text | Google Scholar

114. Sahin-Efe, A, Upadhyay, J, Ko, B-J, Dincer, F, Park, KH, Migdal, A, et al. Irisin and leptin concentrations in relation to obesity, and developing type 2 diabetes: a cross sectional and a prospective case-control study nested in the normative aging study. Metabolism. (2018) 79:24–32. doi: 10.1016/j.metabol.2017.10.011

PubMed Abstract | Crossref Full Text | Google Scholar

115. Li, B, Yao, Q, Guo, S, Ma, S, Dong, Y, Xin, H, et al. Type 2 diabetes with hypertensive patients results in changes to features of adipocytokines: leptin, Irisin, LGR4, and Sfrp5. Clin Exp Hypertens. (2019) 41:645–50. doi: 10.1080/10641963.2018.1529779

PubMed Abstract | Crossref Full Text | Google Scholar

116. Stengel, A, Hofmann, T, Goebel-Stengel, M, Elbelt, U, Kobelt, P, and Klapp, BF. Circulating levels of irisin in patients with anorexia nervosa and different stages of obesity–correlation with body mass index. Peptides. (2013) 39:125–30. doi: 10.1016/j.peptides.2012.11.014

Crossref Full Text | Google Scholar

117. De Meneck, F, de Souza, LV, Oliveira, V, and do Franco, M. High irisin levels in overweight/obese children and its positive correlation with metabolic profile, blood pressure, and endothelial progenitor cells. Nutr Metab Cardiovasc Dis. (2018) 28:756–64. doi: 10.1016/j.numecd.2018.04.009

PubMed Abstract | Crossref Full Text | Google Scholar

118. Komolka, K, Albrecht, E, Schering, L, Brenmoehl, J, Hoeflich, A, and Maak, S. Locus characterization and gene expression of bovine FNDC5: is the myokine irisin relevant in cattle? PLoS One. (2014) 9:e88060. doi: 10.1371/journal.pone.0088060

Crossref Full Text | Google Scholar

119. Albrecht, E, Schering, L, Buck, F, Vlach, K, Schober, H, Drevon, C, et al. Irisin: still chasing shadows. Mol Metab. (2020) 34:124–35. doi: 10.1016/j.molmet.2020.01.016

Crossref Full Text | Google Scholar

120. Kirat, D, Hamada, M, Moustafa, A, and Miyasho, T. Irisin/FNDC5: A participant in camel metabolism. Saudi J Biol Sci. (2021) 28:693–706. doi: 10.1016/j.sjbs.2020.10.061

PubMed Abstract | Crossref Full Text | Google Scholar

121. Basini, G, Bussolati, S, Iannarelli, M, Ragionieri, L, Grolli, S, Ramoni, R, et al. The myokine irisin: localization and effects in swine late medium and large antral ovarian follicle. Domest Anim Endocrinol. (2021) 74:106576. doi: 10.1016/j.domaniend.2020.106576

PubMed Abstract | Crossref Full Text | Google Scholar

122. Kowalik, S, Wiśniewska, A, Kędzierski, W, and Janczarek, I. Concentrations of circulating Irisin and Myostatin in race and Endurace purebred Arabian horses—preliminary study. Animals. (2020) 10:2268. doi: 10.3390/ani10122268

PubMed Abstract | Crossref Full Text | Google Scholar

123. Marrano, N, Biondi, G, Borrelli, A, Cignarelli, A, Perrini, S, Laviola, L, et al. Irisin and incretin hormones: similarities, differences, and implications in type 2 diabetes and obesity. Biomol Ther. (2021) 11:286. doi: 10.3390/biom11020286

PubMed Abstract | Crossref Full Text | Google Scholar

124. Wang, S, and Pan, J. Irisin ameliorates depressive-like behaviors in rats by regulating energy metabolism. Biochem Biophys Res Commun. (2016) 474:22–8. doi: 10.1016/j.bbrc.2016.04.047

PubMed Abstract | Crossref Full Text | Google Scholar

125. Aydin, S, Kuloglu, T, Aydin, S, Kalayci, M, Yilmaz, M, Cakmak, T, et al. A comprehensive immunohistochemical examination of the distribution of the fat-burning protein irisin in biological tissues. Peptides. (2014) 61:130–6. doi: 10.1016/j.peptides.2014.09.014

PubMed Abstract | Crossref Full Text | Google Scholar

126. Xiong, XQ, Chen, D, Sun, HJ, Ding, L, Wang, JJ, Chen, Q, et al. FNDC5 overexpression and irisin ameliorate glucose/lipid metabolic derangements and enhance lipolysis in obesity. Biochim Biophys Acta. (2015) 1852:1867–75. doi: 10.1016/j.bbadis.2015.06.017

PubMed Abstract | Crossref Full Text | Google Scholar

127. So, WY, and Leung, PS. Irisin ameliorates hepatic glucose/lipid metabolism and enhances cell survival in insulin-resistant human HepG2 cells through adenosine monophosphate-activated protein kinase signaling. Int J Biochem Cell Biol. (2016) 78:237–47. doi: 10.1016/j.biocel.2016.07.022

PubMed Abstract | Crossref Full Text | Google Scholar

128. Xin, C, Liu, J, Zhang, J, Zhu, D, Wang, H, Xiong, L, et al. Irisin improves fatty acid oxidation and glucose utilization in type 2 diabetes by regulating the AMPK signaling pathway. Int J Obes. (2016) 40:443–51. doi: 10.1038/ijo.2015.199

PubMed Abstract | Crossref Full Text | Google Scholar

129. Zhang, Y, Li, R, Meng, Y, Li, S, Donelan, W, Zhao, Y, et al. Irisin stimulates browning of white adipocytes through mitogen-activated protein kinase p38 MAP kinase and ERK MAP kinase signaling. Diabetes. (2014) 63:514–25. doi: 10.2337/db13-1106

PubMed Abstract | Crossref Full Text | Google Scholar

130. Lee, TH, Formolo, DA, Kong, T, Lau, SW, Ho, CS, Leung, RYH, et al. Potential exerkines for physical exercise-elicited pro-cognitive effects: insight from clinical and animal research. Int Rev Neurobiol. (2019) 147:361–95. doi: 10.1016/bs.irn.2019.06.002

PubMed Abstract | Crossref Full Text | Google Scholar

131. Ozcan, S, Ulker, N, Bulmus, O, Yardimci, A, Ozcan, M, and Canpolat, S. The modulatory effects of irisin on asprosin, leptin, glucose levels and lipid profile in healthy and obese male and female rats. Arch Phys Biochem. (2022) 128:724–31. doi: 10.1080/13813455.2020.1722706

PubMed Abstract | Crossref Full Text | Google Scholar

132. Majeed, S, Shafi, R, Moin, H, Ashraf, I, Irshad, K, and Liaquat, A. Effects of recombinant irisin on body mass index, serum insulin, luteinizing hormone and testosterone levels in obese female BALB/c mice. J Coll Physicians Surg Pak. (2019) 29:736–40. doi: 10.29271/jcpsp.2019.08.736

PubMed Abstract | Crossref Full Text | Google Scholar

133. Mansour, SW, Hasan, MM, Salah, HE, El-Deep, T, Hussein, S, and El-Malkey, NF. Effect of irisin on metabolic and platelet functions in type 2 diabetic rats: role of soluble receptor of advanced glycation end products (sRAGE). Beni-Suef univ J Basic Appl Sci. (2021) 10:1–7. doi: 10.1186/s43088-021-00148-1

Crossref Full Text | Google Scholar

134. Abozeid, M, and Abeer, A. Potential effect of Irisin and/or moderate intensity exercise on metabolic homeostasis in obesity in male albino rats. Med J Cairo Uni. (2019) 87:5255–62. doi: 10.21608/mjcu.2019.89764

Crossref Full Text | Google Scholar

135. Dehghan, F, Zamani, S, Barreiro, C, and Jami, MS. Irisin injection mimics exercise effects on the brain proteome. Eur J Neurosci. (2021) 54:7422–41. doi: 10.1111/ejn.15493

PubMed Abstract | Crossref Full Text | Google Scholar

136. Huang, L, Yan, S, Luo, L, and Yang, L. Irisin regulates the expression of BDNF and glycometabolism in diabetic rats. Mol Med Rep. (2019) 19:1074–82. doi: 10.3892/mmr.2018.9743

PubMed Abstract | Crossref Full Text | Google Scholar

137. Esposito, G, Irons, PC, Webb, EC, and Chapwanya, A. Interactions between negative energy balance, metabolic diseases, uterine health and immune response in transition dairy cows. Anim Reprod Sci. (2014) 144:60–71. doi: 10.1016/j.anireprosci.2013.11.007

PubMed Abstract | Crossref Full Text | Google Scholar

138. Rumphorst, T, Scheu, T, Koch, C, and Sundrum, A. Balancing trade-offs in Milk production by making use of animal individual energy balancing. Dairy. (2022) 3:345–63. doi: 10.3390/dairy3020027

Crossref Full Text | Google Scholar

139. Ladyman, SR, and Brooks, VL. Central actions of insulin during pregnancy and lactation. J Neuroendocrinol. (2021) 33:e12946. doi: 10.1111/jne.12946

PubMed Abstract | Crossref Full Text | Google Scholar

140. Accorsi, P, Govoni, N, Gaiani, R, Pezzi, C, Seren, E, and Tamanini, C. Leptin, GH, PRL, insulin and metabolic parameters throughout the dry period and lactation in dairy cows. Reprod Domest Anim. (2005) 40:217–23. doi: 10.1111/j.1439-0531.2005.00581.x

PubMed Abstract | Crossref Full Text | Google Scholar

141. Piccione, G, Messina, V, Marafioti, S, Casella, S, Giannetto, C, and Fazio, F. Changes of some haematochemical parameters in dairy cows during late gestation, post partum, lactation and dry periods. Vet Med Zoot. (2012) 58:59–64.

Google Scholar

142. Fiore, E, Piccione, G, Rizzo, M, Morgante, M, Barberio, A, Giudice, E, et al. Adaptation of some energetic parameters during transition period in dairy cows. J Appl Anim Res. (2018) 46:402–5. doi: 10.1080/09712119.2017.1313742

Crossref Full Text | Google Scholar

143. Pascottini, OB, Leroy, JL, and Opsomer, G. Metabolic stress in the transition period of dairy cows: focusing on the prepartum period. Animals. (2020) 10:1419. doi: 10.3390/ani10081419

PubMed Abstract | Crossref Full Text | Google Scholar

144. Ospina, P, Nydam, D, Stokol, T, and Overton, T. Evaluation of nonesterified fatty acids and β-hydroxybutyrate in transition dairy cattle in the northeastern United States: critical thresholds for prediction of clinical diseases. J Dairy Sci. (2010) 93:546–54. doi: 10.3168/jds.2009-2277

PubMed Abstract | Crossref Full Text | Google Scholar

145. Habata, Y, Fujii, R, Hosoya, M, Fukusumi, S, Kawamata, Y, Hinuma, S, et al. Apelin, the natural ligand of the orphan receptor APJ, is abundantly secreted in the colostrum. Biochim Biophys Acta, Mol Cell Res. (1999) 1452:25–35. doi: 10.1016/S0167-4889(99)00114-7

PubMed Abstract | Crossref Full Text | Google Scholar

146. Mesmin, C, Fenaille, F, Becher, F, Tabet, J-C, and Ezan, E. Identification and characterization of apelin peptides in bovine colostrum and milk by liquid chromatography–mass spectrometry. J Proteome Res. (2011) 10:5222–31. doi: 10.1021/pr200725x

PubMed Abstract | Crossref Full Text | Google Scholar

147. Moschen, AR, Kaser, A, Enrich, B, Mosheimer, B, Theurl, M, Niederegger, H, et al. Visfatin, an adipocytokine with proinflammatory and immunomodulating properties. J Immunol. (2007) 178:1748–58. doi: 10.4049/jimmunol.178.3.1748

PubMed Abstract | Crossref Full Text | Google Scholar

148. Lemor, A, Hosseini, A, Sauerwein, H, and Mielenz, M. Transition period-related changes in the abundance of the mRNAs of adiponectin and its receptors, of visfatin, and of fatty acid binding receptors in adipose tissue of high-yielding dairy cows. Domest Anim Endocrinol. (2009) 37:37–44. doi: 10.1016/j.domaniend.2009.01.004

PubMed Abstract | Crossref Full Text | Google Scholar

149. Li, X, Fu, X, Yang, G, and Du, M. Enhancing intramuscular fat development via targeting fibro-adipogenic progenitor cells in meat animals. Animal. (2020) 14:312–21. doi: 10.1017/S175173111900209X

PubMed Abstract | Crossref Full Text | Google Scholar

150. Rashid, FA, Abbas, HJ, Naser, NA, and Ali, A. Effect of long-term moderate physical exercise on irisin between normal weight and obese men. Sci World J. (2020) 2020:1–7. doi: 10.1155/2020/1897027

PubMed Abstract | Crossref Full Text | Google Scholar

151. Li, L, Yang, G, Li, Q, Tang, Y, Yang, M, Yang, H, et al. Changes and relations of circulating visfatin, apelin, and resistin levels in normal, impaired glucose tolerance, and type 2 diabetic subjects. Exp Clin Endocrinol Diabetes. (2006) 114:544–8. doi: 10.1055/s-2006-948309

PubMed Abstract | Crossref Full Text | Google Scholar

152. Roche, J, Ramé, C, Reverchon, M, Mellouk, N, Rak, A, Froment, P, et al. Apelin (APLN) regulates progesterone secretion and oocyte maturation in bovine ovarian cells. Reproduction. (2017) 153:589–603. doi: 10.1530/REP-16-0677

PubMed Abstract | Crossref Full Text | Google Scholar

153. Rak, A, Drwal, E, Rame, C, Knapczyk-Stwora, K, Słomczyńska, M, Dupont, J, et al. Expression of apelin and apelin receptor (APJ) in porcine ovarian follicles and in vitro effect of apelin on steroidogenesis and proliferation through APJ activation and different signaling pathways. Theriogenology. (2017) 96:126–35. doi: 10.1016/j.theriogenology.2017.04.014

PubMed Abstract | Crossref Full Text | Google Scholar

154. Shokrollahi, B, Zheng, H-Y, Li, L-Y, Tang, L-P, Ma, X-Y, Lu, X-R, et al. Apelin and apelin receptor in follicular granulosa cells of buffalo ovaries: expression and regulation of steroidogenesis. Front Endocrinol. (2022) 13:844360. doi: 10.3389/fendo.2022.844360

PubMed Abstract | Crossref Full Text | Google Scholar

155. Gupta, M, Korde, JP, Bahiram, K, Sardar, V, and Kurkure, NV. Expression and localization of apelin and apelin receptor (APJ) in buffalo ovarian follicles and corpus luteum and the in-vitro effect of apelin on steroidogenesis and survival of granulosa cells. Theriogenology. (2023) 197:240–51. doi: 10.1016/j.theriogenology.2022.12.013

PubMed Abstract | Crossref Full Text | Google Scholar

156. Shokrollahi, B, Zheng, H-Y, Ma, X-Y, and Shang, J-H. The effects of apelin on IGF1/FSH-induced steroidogenesis, proliferation, Bax expression, and total antioxidant capacity in granulosa cells of buffalo ovarian follicles. Vet Res Commun. (2023) 47:1523–33. doi: 10.1007/s11259-021-09799-4

Crossref Full Text | Google Scholar

157. Reverchon, M, Rame, C, Bunel, A, Chen, W, Froment, P, and Dupont, J. VISFATIN (NAMPT) improves in vitro IGF1-induced steroidogenesis and IGF1 receptor signaling through SIRT1 in bovine granulosa cells. Biol Reprod. (2016) 94:54. doi: 10.1095/biolreprod.115.134650

Crossref Full Text | Google Scholar

158. Diot, M, Reverchon, M, Rame, C, Froment, P, Brillard, J-P, Brière, S, et al. Expression of adiponectin, chemerin and visfatin in plasma and different tissues during a laying season in turkeys. Reprod Biol Endocrinol. (2015) 13:1–14. doi: 10.1186/s12958-015-0081-5

Crossref Full Text | Google Scholar

159. Thakre, A, Gupta, M, Magar, S, Bahiram, K, Sardar, V, Korde, J, et al. Transcriptional and translational abundance of visfatin (NAMPT) in buffalo ovary during estrous cycle and its in vitro effect on steroidogenesis. Domest Anim Endocrinol. (2021) 75:106583. doi: 10.1016/j.domaniend.2020.106583

PubMed Abstract | Crossref Full Text | Google Scholar

160. Sato, K, Takahashi, T, Kobayashi, Y, Hagino, A, Roh, S, and Katoh, K. Apelin is involved in postprandial responses and stimulates secretion of arginine-vasopressin, adrenocorticotropic hormone, and growth hormone in the ruminant. Domest Anim Endocrinol. (2012) 42:165–72. doi: 10.1016/j.domaniend.2011.11.006

PubMed Abstract | Crossref Full Text | Google Scholar

161. Bayraktar, B, Tekce, E, Aksakal, V, Takma, Ç, Bayraktar, FG, and Şengül, B. Effects of race, gender, body condition score and pregnancy on serum Apelin levels in ewe. J Agric Sci. (2020) 26:363–72. doi: 10.15832/ankutbd.526907

Crossref Full Text | Google Scholar

162. Aydin, S . Presence of adropin, nesfatin-1, apelin-12, ghrelins and salusins peptides in the milk, cheese whey and plasma of dairy cows. Peptides. (2013) 43:83–7. doi: 10.1016/j.peptides.2013.02.014

PubMed Abstract | Crossref Full Text | Google Scholar

Keywords: apelin, visfatin, irisin, energy regulation, farm animals

Citation: Shokrollahi B, Jang S-S, Lee HJ, Ahmad HI, Sesay AR, Ghazikhani Shad A, Morammazi S and Abdelnour SA (2024) Exploring the potential roles of apelin, visfatin, and irisin in energy regulation in farm animals: an overview. Front. Vet. Sci. 11:1435788. doi: 10.3389/fvets.2024.1435788

Received: 21 May 2024; Accepted: 05 July 2024;
Published: 19 July 2024.

Edited by:

Elena De Felice, University of Camerino, Italy

Reviewed by:

Francesca Mercati, University of Perugia, Italy
Cecilia Dall’Aglio, University of Perugia, Italy
Paola Scocco, University of Camerino, Italy

Copyright © 2024 Shokrollahi, Jang, Lee, Ahmad, Sesay, Ghazikhani Shad, Morammazi and Abdelnour. This is an open-access article distributed under the terms of the Creative Commons Attribution License (CC BY). The use, distribution or reproduction in other forums is permitted, provided the original author(s) and the copyright owner(s) are credited and that the original publication in this journal is cited, in accordance with accepted academic practice. No use, distribution or reproduction is permitted which does not comply with these terms.

*Correspondence: Borhan Shokrollahi, Borhansh@gmail.com

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