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Review

The Molecular Mechanisms of Fuel Utilization during Exercise

by
Anna Pi
,
Sneha Damal Villivalam
and
Sona Kang
*
Nutritional Sciences and Toxicology Department, University of California Berkeley, Berkeley, CA 94720, USA
*
Author to whom correspondence should be addressed.
Biology 2023, 12(11), 1450; https://doi.org/10.3390/biology12111450
Submission received: 29 September 2023 / Revised: 16 November 2023 / Accepted: 17 November 2023 / Published: 19 November 2023
Versions Notes

Abstract

:

Simple Summary

Exercise has well-known health benefits, but the way our muscles use carbohydrates and lipids as fuel during exercise is complex. It is not just about the physical activity itself; it also depends on our body’s metabolic state. The balance between using carbs and fats affects exercise performance. This review aims to provide a comprehensive look at how our bodies choose fuel sources during exercise by summarizing existing research. Understanding this can lead to advancements in exercise science and personalized exercise strategies for better health and performance.

Abstract

Exercise is widely recognized for its positive impact on human health and well-being. The process of utilizing substrates in skeletal muscle during exercise is intricate and governed by complex mechanisms. Carbohydrates and lipids serve as the primary fuel sources for skeletal muscle during exercise. It is now understood that fuel selection during exercise is not solely determined by physical activity itself but is also influenced by the overall metabolic state of the body. The balance between lipid and carbohydrate utilization significantly affects exercise capacity, including endurance, fatigue, and overall performance. Therefore, comprehensively understanding the regulation of substrate utilization during exercise is of utmost importance. The aim of this review is to provide an extensive overview of the current knowledge regarding the pathways involved in the regulation of substrate utilization during exercise. By synthesizing existing research, we can gain a holistic perspective on the intricate relationship between exercise, metabolism, and fuel selection. This advanced understanding has the potential to drive advancements in the field of exercise science and contribute to the development of personalized exercise strategies for individuals looking to optimize their performance and overall health.

1. Introduction

Exercise is increasingly recognized as a vital component for achieving optimal health and promoting extended life expectancy. Numerous studies have proven that physical exercise has positive effects on human health and may have both preventative and mitigating effects on chronic diseases such as diabetes and cardiovascular disease [1]. The majority of our movement and contraction during exercise is attributed to our skeletal muscles [2].
Exercise can generally be classified into two main categories: endurance exercise and resistance exercise. However, it is important to note that many activities often involve a combination of both endurance and resistance components. Endurance (aerobic) exercise refers to types of physical activity performed at a lower intensity over a longer duration, such as long-distance running and swimming [3]. Resistance (strength-based) exercise refers to types of physical activity which are performed at a higher intensity over a shorter duration, such as weightlifting [3]. The benefits of exercise depend on the type of physical activity performed. Endurance training has been associated with notable improvements in cardiac output, oxygen consumption, and mitochondrial biogenesis [2]. On the other hand, resistance exercise has been demonstrated to increase muscle size, enhance neural adaptations, and improve overall strength [2]. Endurance exercise is effective in reducing cardiovascular risk factors, while resistance exercise helps maintain metabolic rate, muscle mass, and physical function with age [2]. A combination of endurance and resistance exercise has been demonstrated to induce insulin resistance and enhance glycemic control in chronic diseases like type 2 diabetes (T2D) and obesity [4,5]. The effects of exercise also depend upon duration. Acute exercise, or a single bout of exercise, results in increases in muscle protein synthesis [6] and insulin sensitivity [7]. Chronic exercise, which is exercise performed over weeks or longer, builds on the muscle-specific benefits of acute exercise and induces more peripheral insulin sensitivity [8], as well as increasing muscle mass and maximal oxygen consumption [8,9,10].
During exercise, skeletal muscle primarily relies on various fuel sources to meet its energy demands. Glucose, lipids, and, to a lesser extent, amino acids are the key contributors to this energy production [10]. Muscle glycogen is particularly critical during high-intensity activities as it provides an immediate source of glucose, allowing for quick bursts of energy [2,10]. Simultaneously, the liver plays a crucial role in maintaining blood glucose levels by releasing glucose into the bloodstream, ensuring a stable supply of this essential energy source [2,10].
It is important to note that lipid utilization is not limited to high-intensity activities; it extends to a broader spectrum of exercise intensities. However, during exercise, there is reduced lipolysis, the process of breaking down stored fat into fatty acids for energy, which can limit the contribution of lipids as a primary fuel source [2,10]. Nevertheless, lipid sources such as intramuscular triglycerides (IMTGs) and ketones play vital roles in energy production. IMTGs, stored within muscle cells, serve as a readily available source of energy, especially during endurance activities [2,10]. Additionally, ketone bodies, including beta-hydroxybutyrate and acetoacetate, produced by the liver, can be utilized during exercise, particularly when glucose availability is limited [2,10]. Furthermore, amino acids can serve as an energy source, which becomes particularly significant during prolonged or high-intensity exercise when glycogen and glucose stores become depleted. Amino acids can be derived from both muscle protein breakdown and circulating amino acids in the blood [2,10]. This dynamic interplay among glucose, lipids (including IMTGs and ketones), and amino acids adapts to the exercise’s intensity and duration, ensuring a continuous supply of energy to sustain muscle contractions and meet the ever-changing demands of physical activity.
The ability to smoothly transition between these fuel sources, especially glucose to lipids, is known as “metabolic flexibility” [11]. However, individuals with obesity or T2D often exhibit “metabolic inflexibility”, characterized by an impaired ability to efficiently switch between fuel sources [12]. In this review, we will delve into the significance of fuel utilization in exercise performance, focusing specifically on insights gained from genetic mouse studies.

2. Lipid Utilization

2.1. Factors Regulating Substrate Availability

Skeletal muscle expresses several fatty acid transporters, including the plasma membrane fatty acid-binding protein (FABPpm), fatty acid transport protein (FATP) 1 and 4 and fatty acid translocase CD36 (FAT/CD36) [13]. It has been shown that CD36 is critical to mediate fatty acid transport and fatty acid oxidation in skeletal muscles [14,15]. Studies by Manio et al. demonstrated that Cd36 whole-body knockout mice exhibited a significant reduction (44%) in their ability to sustain exercise at a submaximal running speed [14,15]. This decline was attributed to the loss of CD36-mediated fatty acid transport into the muscle, leading to metabolic inflexibility—the inability to smoothly switch from glucose to fatty acid utilization during exercise. However, no changes in muscle mitochondrial enzymes and biogenesis were observed [14,15]. Studies have shown beneficial changes in whole-body metabolism in Fatp1 whole-body knockout (KO) mice, though its specific role in exercise performance has not yet been reported [16]. Fabp4/Fabp5 double knockout mice have also been shown to have decreased endurance exercise capacity when fasted compared to WT mice [17].
Low to moderate physical exercise triggers the process of lipolysis in white adipose tissue (WAT), releasing free fatty acids as a source of fuel [18]. Adipose triacylglycerol lipase (ATGL) and hormone-sensitive lipase (HSL) are the two primary enzymes responsible for triacylglycerol (TG) hydrolysis in adipose tissue. These enzymes account for approximately 95% of TG lipase activity, breaking down TG into diacylglycerol and further converting DG into monoacylglycerol [19]. Studies have demonstrated the essential role of ATGL and HSL in supplying free fatty acids during endurance exercise in mice. KO mice lacking Atgl or Hsl exhibited reduced exercise capacity. These mice failed to promote exercise-induced lipolysis and showed increased carbohydrate oxidation during exercise, leading to faster depletion of muscle and liver glycogen [19,20]. Collectively, these findings highlight the critical role of regulating free fatty acid availability for optimal endurance exercise performance.
Carnitine acts as a cofactor for enzymes such as carnitine translocase and acylcarnitine transferases I and II, which are vital for converting free long-chain fatty acids into acylcarnitines and transporting them into the mitochondrial matrix [21]. Fatty acid oxidation occurs before these substrates enter the Krebs cycle, where energy production takes place [21]. Since mitochondria membranes are impermeable to CoA esters and long-chain fatty acids, the binding of L-carnitine to acetyl groups through carnitine acyltransferase is crucial for transporting acetylated fatty acids into the mitochondria and facilitating their subsequent oxidation in the matrix [22]. A study by Kim et al. administered 150 mg/kg body weight of L-Carnitine orally to C57BL/6 wild-type mice over a three-week exercise training period. The findings revealed significant increases in mRNA and protein expression of key regulators involved in fatty acid oxidation and mitochondrial biogenesis in skeletal muscle. This enhancement in gene expression was associated with improved exercise endurance. Furthermore, the study observed a preservation of both protein and carbohydrate utilization during exercise, emphasizing the significance of optimal fuel utilization in promoting endurance exercise capacity [23].
Vascular endothelial growth factor (VEGF) plays a crucial role in promoting vasculogenesis and angiogenesis, thereby increasing blood supply to various tissues [24]. In the context of adipose tissue, VEGF facilitates the delivery of nutrients and oxygen to adipose tissue and enables the transportation of fatty acids to other parts of the body as energy substrates [24,25]. Elevated levels of circulating VEGF have been observed in obese individuals, prompting studies to investigate the role of VEGF in obesity and metabolic health through the generation of adipocyte-specific Vegf KO (adipo-Vegf KO) mice [25]. Remarkably, adipo-Vegf KO mice demonstrated impaired exercise tolerance, as well as hypoinsulinemia, hypoglycemia, and lower serum free fatty acid levels compared to control mice [25]. These KO mice also exhibited a significant decline of up to 40% in adipose capillarity [25]. The authors hypothesized that the reduction in capillaries compromised the transport of lipids from adipose tissue to skeletal muscle, thereby impairing the availability of fuel for endurance exercise and ultimately leading to decreased exercise endurance in the adipo-Vegf KO mice [25]. This finding supports the notion that the bioavailability of free fatty acids from adipose tissue is crucial for supporting optimal endurance exercise performance.

2.2. Factors Regulating Mitochondrial Biology

During muscle contraction, a significant portion of the required ATP is generated by mitochondria through a process called oxidative phosphorylation [26]. The effects of exercise on mitochondrial dynamics and functions vary depending on the intensity and type of exercise, often involving the regulation of proteins associated with mitochondrial pathways. Exercise can stimulate the upregulation of mitochondrial biogenesis and influence the morphology of mitochondria through fusion and fission processes, ultimately impacting mitochondrial oxidative capacity [27].
Optic atrophy 1 (OPA1) is a dynamin family member found in the inner mitochondrial membrane which regulates mitochondrial fusion [28]. It also plays a role in mitochondrial biogenesis by facilitating fusion of inner mitochondrial membranes and formation of cristae [29], particularly during physiological stresses like endurance training [30]. Surprisingly, Opa1 haplodeficient mice exhibited reduced mitochondrial mass, lower activity of citrate synthase and cytochrome oxidase, and abnormal cristae morphology [30]. However, these mice demonstrated significantly improved endurance capacity after training, without changes in training capacity. This enhancement may be attributed to compensatory mechanisms such as increased levels of carnitine palmitoyltransferase 2, an enzyme essential for fatty acid oxidation, leading to enhanced fatty acid utilization [30]. Nuclear factor erythroid 2-related factor 2 (NRF2) is a transcription factor involved in cellular defense against oxidative stress and toxins by regulating target genes. Acute high-intensity interval exercise has been shown to activate NRF2 signaling in humans [31]. Nrf2 deficiency has been linked to skeletal muscle mitochondrial defects, including reduced content and impaired oxidative phosphorylation, leading to impaired exercise endurance in NRF2 KO mice [31]. Kelch-like ECH-associated protein 1 (KEAP1) is a negative regulator of NRF2, responsible for its degradation under normal conditions [32]. Muscle-specific Keap1 KO mice exhibited improved endurance and resistance exercise capacity. These KO mice showed increased mitochondrial content, succinate dehydrogenase activity, and enhanced mobilization and oxidation of fatty acids during exercise. Metabolic profiling revealed reduced nucleoside triphosphates, including ATP production, possibly due to mitochondrial uncoupling or increased ATP consumption [32]. Another study, which used sulforaphane (SFN) as an NRF2 inducer to stimulate NRF2 signaling, also discovered that this stimulation resulted in an enhanced exercise capacity [33]. Reactive oxygen species (ROS) are known to increase in skeletal muscles during exercise. However, the exact effects of ROS are still debated since both insufficient ROS production and overproduction of ROS can impact exercise ability [34]. Biomarker measurements for oxidative stress and muscle damage decreased in mice that were pretreated with SFN. Downstream target genes of NRF2 included many antioxidant genes such as HO-1, NQO1, γ-GCS, and catalase [33]. The increased expression of NRF2 target genes in muscle suggests that the NRF2 pathway plays a vital role in fuel utilization during exercise [32] and regulating oxidative stress [33].
Peroxisome proliferator-activated receptor gamma coactivator 1-alpha (PGC-1a) is a co-transcription factor that plays a crucial role in regulating various metabolic pathways [35]. PGC-1a is involved in promoting fatty acid oxidation, mitochondrial function, and mitochondrial biogenesis [36]. Studies have demonstrated that whole-body KO mice lacking Ppargc1a exhibit impaired glucose homeostasis, altered hepatic energy metabolism, reduced expression of genes related to mitochondrial function, and exercise intolerance [35,37]. Similarly, muscle-specific Pgc1a KO mice have been shown to have a higher proportion of fast-twitch fibers and display exercise intolerance under basal conditions [38]. Conversely, muscle-specific Pgc1a transgenic mice exhibit a higher proportion of slow-twitch fibers, which are rich in mitochondria and more resistant to fatigue [39,40]. However, two additional independent studies using muscle-specific Pgc1a KO mice reported that PGC-1a is not essential for mediating voluntary exercise, although the impact of Pgc1a deficiency on exercise-induced mitochondrial biogenesis varied between the studies [41,42]. In humans, exercise induces a transient increase in PGC-1a mRNA levels [43,44], though there are conflicting results in how well mRNA changes reflect protein levels; one study found a significant increase in PGC-1a protein level directly after prolonged exercise [44] while two others did not [45,46].
SESTRINs (SESN1, 2, and 3) are stress-induced proteins that play important roles in various biological processes. It was shown that SESN2 and SESN3 levels increase in response to exercise in both mice and humans [47,48,49]. Overexpression of SESTRINs in flies has been shown to mimic many of the beneficial effects of exercise [50]. Studies using whole-body Sesn triple KO mice, which lack all three isoforms, have shown that these mice have decreased endurance capacity, impaired insulin sensitivity, and reduced mitochondrial biogenesis in muscle [50]. Mice that had whole-body KO of Sesn1, the primary isoform expressed in skeletal and cardiac muscles, demonstrated a decreased exercise capacity and a preference for glucose utilization during exercise, as indicated by a gradual increase in the respiratory exchange ratio (RER) [50], which is a method of measuring CO2 and O2 consumption to determine whether lipid or carbohydrate consumption is preferentially used [51,52]. The activation of SESN is thought to mimic the effects of exercise through two primary downstream pathways. First, SESNs can activate TORC2, which in turn activates AKT signaling. This facilitates insulin-dependent glucose and fat utilization, as well as the maintenance of muscle mass. Second, SESNs upregulate AMPK signaling, leading to increased levels of PGC-1a through both transcriptional and post-transcriptional mechanisms [50]. Overall, the activation of SESN during exercise appears to contribute to improved metabolic outcomes by regulating multiple signaling pathways involved in glucose and fat utilization, muscle mass maintenance, and mitochondrial biogenesis.

2.3. Transcription Factors

Peroxisome proliferator-activated receptor alpha (PPARα) plays a crucial role in regulating lipid and glucose metabolism [53]. Studies in both mice and humans have reported an increase in PPARα expression following exercise [54,55,56]. Investigations using whole-body Ppara KO mice have shown these mice have a reduction in basal fatty acid oxidation and impaired response to AICAR treatment, an AMPK activator [57,58]. Additionally, the KO mice exhibited lower levels of muscle palmitate oxidation at rest. Conversely, muscle-specific overexpression of PPARα resulted in elevated muscle palmitate oxidation and decreased expression of genes involved in glucose utilization, such as GLUT1 and GLUT4 [58]. The downregulation of these genes may be linked to the disruption of MEF2A/PGC-1α-dependent control of GLUT4 gene expression. However, there have been discrepancies between studies regarding the impact of Ppara deficiency on fatty acid oxidation and PPARα target gene expression in skeletal muscle [54,57,58]. These inconsistencies may be attributed to differences in the genetic backgrounds of the mice used. It is worth noting that while whole-body Ppara KO mice did not display significant changes in fatty acid oxidation or PPARα target gene expression, they did exhibit reduced exercise endurance and increased liver glycogen depletion [54]. This suggests that compensatory mechanisms, potentially involving high levels of PPARδ in skeletal muscle, may partially offset the loss of PPARα function. Further investigation using muscle-specific conditional KO mice will be essential in clarifying PPARα’s precise role in fuel utilization during exercise. In summary, the studies indicate that PPARα plays a vital role in exercise performance by promoting lipid utilization over glucose through the enhancement of fatty acid oxidation in skeletal muscle. Its activation during exercise may contribute to the metabolic adaptations required for efficient energy utilization during physical activity.
KLF15 is a transcription factor highly expressed in metabolic tissues and plays a crucial role in regulating macronutrient metabolism [59]. It is upregulated in skeletal muscle after exercise and particularly enriched in oxidative soleus muscle [60]. Whole-body Klf15 KO mice exhibit reduced exercise endurance and impaired metabolic gene expression related to fatty acid utilization and mitochondrial function [60]. The skeletal muscle of KO mice shows mitochondrial defects and altered fuel utilization during exercise, with decreased lipid oxidation and increased carbohydrate usage. However, compensatory changes in gene expression related to lipid metabolism are observed. These findings highlight the importance of KLF15 in coordinating fuel utilization in skeletal muscle during exercise.
The nuclear receptor 4A1 (NR4A1), also known as NUR77, is a transcription factor preferentially expressed in fast-twitch muscle fibers, which contain fewer mitochondria and fatigue more quickly than slow-twitch fibers [39,40,61]. Studies have shown that Nur77 expression is robustly induced by β-adrenergic stimulation and physical exercise [61]. Muscle-specific Nur77 transgenic mice were generated, and unexpectedly, their Nur77 transgenic muscle had an increased abundance of slow-twitch oxidative muscle fibers and mitochondrial DNA content [62]. These muscles also exhibited enhanced oxidative metabolism, indicating increased mitochondrial activity [62]. Metabolomic analysis confirmed that Nur77 transgenic muscle favored fatty acid oxidation over glucose oxidation, resembling the metabolic profile of fasting [62]. Nur77 expression also improved the intrinsic respiratory capacity of isolated mitochondria, likely due to increased abundance of complex I of the electron transport chain [62]. These changes in mitochondrial metabolism translated to improved muscle contractile function ex vivo [62]. Overall, this study highlights a novel role for NUR77 in regulating oxidative metabolism and mitochondrial activity in skeletal muscle.
Nuclear factor-κB (NF-κB) is a transcription factor composed of different subunits ([p50, p52, p65 (RelA), RelB, and c-Rel]) that regulate gene expression [63,64,65]. Studies have demonstrated that endurance exercise reduces NF-κB activation, leading to beneficial effects on skeletal muscle, such as mitochondrial adaptations and prevention of protein degradation [63,64,65]. Whole-body KO mice lacking the p50 subunit of NF-κB exhibited improved long-term endurance and a lower RER during running exercise compared to wild-type mice [64]. These knockout mice also showed higher muscle glycogen levels and lower lactate production from carbohydrate metabolism after running [64]. The study suggests that the effects of p50 deficiency on fuel utilization and exercise performance may be attributed to the inhibitory action of p50 on the transcriptional activity of PPARα and PPARδ.

2.4. Extracellular Factors

IL-13 is a prominent Th2 cytokine that is classified as an anti-inflammatory cytokine due to its ability to suppress the secretion of several macrophage and monocyte-derived inflammatory cytokines [66]. A study showed that whole-body Il13 KO mice demonstrated reduced running capacity on a treadmill relative to wild-type control animals [67]. Furthermore, these KO mice failed to increase the expression of mitochondrial and fatty acid oxidation genes in skeletal muscle in response to exercise. Moreover, Il13-KO mice had muscle that showed defective fatty acid utilization after a single bout of exercise and failed to increase mitochondrial biogenesis after endurance training. Mechanistically, it was shown that IL-13 is required to mediate active phosphorylation of STAT3, which is known to be important for performing full capacity endurance exercise. It was also found that IL13-STAT3 signaling activates several mitochondrial genes through ERRɑ and ERRg, which are orphan receptors known to regulate fatty acid catabolism and mitochondrial respiration in muscle. This study highlights the important role of IL-13 in energy substrate utilization during endurance exercise.

3. Glucose Utilization

3.1. Factors Regulating Substrate Availability

Long-chain acyl-CoA synthetases (ACSLs) convert long-chain fatty acids to fatty acyl-CoAs for oxidation. ACSL1, found in highly oxidative tissues like the outer mitochondrial membrane, facilitates the entry of fatty acids into mitochondria for β-oxidation [68]. Muscle-specific KO of Acsl1 (Acsl1M−/−) in mice leads to reduced β-oxidation in muscles, resulting in a significant decrease in endurance exercise capacity [69]. Although glycogen and triacylglycerol stores remain similar, Acsl1M−/− mice exhibit lower plasma glucose concentrations and a higher RER [69], indicating an increased reliance on glucose as a fuel source. This shift towards glucose usage may be attributed to the depletion of glucose reserves caused by excessive glucose utilization and potential utilization of amino acids as fuel within the muscle, limiting substrate availability for hepatic gluconeogenesis [69]. Thus, impaired conversion of long-chain acyl-CoA to fatty acyl-CoAs and their transport into the mitochondrial matrix in skeletal muscle contributes to excessive glucose utilization.
Glycogen synthase (GYS) is an essential enzyme for glycogen synthesis in skeletal muscle [70]. There are two isoforms of GYS in mammals: GYS2, primarily expressed in the liver, and GYS1, expressed in skeletal and cardiac muscle, as well as other tissues [71]. A study utilizing muscle-specific Gys1 KO mice (Gys1-KO) revealed the significant role of GYS1 in muscle glycogen synthesis and non-oxidative glucose metabolism. The Gys1-KO mice exhibited peripheral insulin resistance, glucose intolerance, and impaired muscle function during contraction and exercise, which affected their endurance capacity [72]. The lack of Gys1 led to muscle glycogen depletion, resulting in reduced muscle performance and fatigue during exercise [72]. Additionally, the Gys1-KO mice showed decreased glucose turnover, impaired muscle glucose uptake, elevated plasma and muscle lactate levels, and reduced levels of muscle hexokinase II [72], indicating peripheral insulin resistance. These findings highlight the critical role of GYS1 in maintaining muscle glycogen levels, muscle function, and glucose metabolism during exercise.
Apoptosis-inducing mitochondrion-associated factor 2 (AIFM2) is an NADH/NAD+ oxidoreductase belonging to the apoptosis-inducing factor (AIF) protein family [73]. AIFM2 expression is significantly increased in glycolytic fast-twitch muscles during high-intensity exercise [74]. Studies using muscle-specific knockdown (KD) or haploinsufficiency of Aifm2 in mice demonstrated reduced exercise capacity accompanied by elevated plasma glucose levels and decreased plasma free fatty acid levels [74], indicating impaired glucose utilization. These mice also exhibited a lower NAD+/NADH ratio after exercise [74]. Conversely, overexpression of AIFM2 in the fast-twitch muscles resulted in improved exercise capacity, enhanced glucose utilization, decreased fatty acid oxidation, and an increased NAD+/NADH ratio after exercise [74]. Delivery of NDE1, an external NADH oxidoreductase, reversed the exercise defects in muscle-specific Aifm2 haploinsufficient mice by restoring the NAD+ ratio, increasing exercise capacity by approximately 30% and normalizing glucose and fatty acid utilization [74]. These findings highlight the physiological role of AIFM2 in promoting glycolysis during high-intensity exercise by facilitating NAD+ availability through its NADH oxidoreductase function.

3.2. Signaling Factors

S6K1, a component of the mTORC1 signaling pathway, regulates cell growth and muscle mass [75]. Resistance training activates mTORC1, leading to increased S6K1 phosphorylation and muscle hypertrophy. S6k1 KO mice are protected against insulin resistance and glucose intolerance [75]. After exercise training, S6k1 KO mice exhibit enhanced running capacity, reduced triglyceride levels in the liver and muscle, and increased ketogenesis [75]. This suggests improved lipid utilization and preservation of glycogen reserves. The absence of S6K1 mimics the effects of chronic endurance exercise, promoting efficient substrate utilization and carbohydrate conservation during high-fat diet consumption.
mTORC1 activity is regulated by interactions with GTPases, including RHEB and RAGs, which enable mTORC1 to localize to the lysosome for its kinase activity [76]. GATOR1, composed of NPRL2, NPRL3, and DEPDC5, acts as a negative regulator of RAG and prevents mTORC1 translocation to the lysosome during amino acid limitation [77]. Muscle-specific Nprl2 KO mice exhibit hyperactive mTORC1 signaling, leading to an increase in glycolytic fibers and a higher RER during exercise [76]. These mice also show decreased expression of Pgc1α, a regulator of mitochondrial biogenesis, and increased expression of glucose uptake-related genes [76]. The activation of mTORC1 promotes mitochondrial amino acid synthesis, resulting in increased glycolysis to meet ATP demands. Similarly, muscle-specific Depdc5 KO mice demonstrate constitutive mTORC1 activation and a tendency towards increased glycolytic muscle fibers [77]. These mice exhibit heightened mitochondrial respiratory capacity without improved endurance, indicating hyperactive mitochondria in glycolytic muscles [77]. Overall, the GATOR1 complex and mTORC1 play crucial roles in regulating carbohydrate utilization and maintaining mitochondrial homeostasis in skeletal muscle. Simultaneous activation of both RHEB and RAG via muscle-specific Tsc1/Depdc5-double knockout can lead to early-onset myopathy associated with excessive mitochondrial oxidative stress. They also showed cardiovascular defects and early fatality, further emphasizing the role of mTORC1 in mediating mitochondrial function and maintaining homeostasis [78].
AMPK is a kinase involved in energy metabolism and gene transcription, acting as a whole-body stress sensor [79,80]. It is activated in response to energy-depleting conditions and integrates signals from exercise, nutrients, and hormones to regulate food intake, energy expenditure, and substrate usage [81]. AMPK consists of α, β, and γ subunits, with the β subunits playing a critical role in assembling the heterotrimer and regulating enzyme activity and localization [80]. In skeletal muscle, α2β2γ3-containing heterotrimers are predominant. KO mice lacking β1 and β2 subunits (β1β2m-KO) show reduced physical activity and impaired treadmill running capacity, accompanied by decreased skeletal muscle mitochondrial content [80]. Notably, β1β2m-KO mice fed a normal diet do not exhibit changes in body weight or insulin sensitivity but display impaired glucose uptake during muscle contractions, indicating the importance of AMPK in glucose utilization [80]. Further research is needed to fully understand the precise role of AMPK in skeletal muscle.

3.3. Transcription Factors

PPARδ is a nuclear receptor that plays a crucial role in regulating fatty acid metabolism in muscle. PPARδ overexpression in skeletal muscle promotes the transformation of muscle fibers to an oxidative type and enhances fatty acid oxidation by increasing the expression of two important mitochondrial proteins: carnitine palmitoyl-transferase 1b and pyruvate dehydrogenase kinase isozyme 4 [82]. This metabolic adaptation is dependent on muscle PPARδ and can be stimulated by PPARδ ligands [82]. Importantly, higher expression of muscle PPARδ is associated with improved endurance performance. Additionally, PPARδ activation suppresses glucose breakdown without affecting muscle fiber type or mitochondrial content [82]. By preserving glucose levels, PPARδ helps to delay the onset of low blood sugar and significantly prolong running time in treated mice [82]. These findings highlight the dual role of PPARδ in promoting glucose sparing and suggest the potential use of PPARδ-targeted exercise mimetics in treating metabolic disorders, muscular dystrophies, and potentially enhancing athletic performance.
The myogenic transcription factor Myogenin is crucial for the development of skeletal muscle during embryonic and fetal stages [83]. Surprisingly, inducible whole-body Myog KO mice at 12 weeks of age exhibited normal muscle development but showed improved performance compared to controls in both high- and low-intensity treadmill running [83]. This enhanced exercise capacity was attributed to more efficient oxidative metabolism during low- and high-intensity exercise, as well as more efficient glycolytic metabolism during high-intensity exercise [83]. Notably, Myog deletion resulted in excessive depletion of blood glucose during intense exercise [83]. Additionally, Myog KO mice displayed higher trainability in voluntary exercise training on running wheels [83], suggesting that Myogenin plays a critical role in regulating the balance between aerobic and anaerobic metabolism in adult skeletal muscle.
Hypoxia-Inducible Factor (HIF)-1α plays an integral role in the body’s response to low oxygen concentrations, or hypoxia [84]. During exercise, hypoxia influences important aspects of muscle function, including ATP production, energy substrate utilization, and the generation of metabolites that contribute to fatigue [85]. Glycolysis, the anaerobic energy pathway, is regulated by HIF-1a under conditions of low oxygen availability [85]. Muscle-specific Hif1a KO mice exhibited a shift in fuel utilization from glucose to lipid oxidation. They demonstrated resistance to the exercise-induced activation of genes involved in glycolysis and glucose uptake, such as Pfkm, Glut4, Pgk, and Ldha [85]. During exercise, the KO mice had reduced levels of serum lactate, indicating decreased reliance on glycolysis [86] while mitochondrial activity increased [85]. However, repeated exercise led to shorter exercise times in the knockout mice compared to the control group, primarily due to extensive muscle damage [85]. Additionally, the KO mice displayed severe impairments in skeletal muscle glycogenolysis and glycolysis [85]. Overall, this study highlights the role of HIF-1a in promoting glucose utilization over lipid utilization during exercise.

3.4. Extracellular Factors

IL-6 was the first myokine discovered to be released into the bloodstream in response to muscle contractions [87] and is one of the most extensively studied exerkines [88]. Its concentration can increase up to 100-fold during exercise. Studies using whole-body Il6 KO mice have shown that these mice have reduced endurance capacity compared to wild-type mice [89]. This reduced endurance is accompanied by significant intramuscular glycogen depletion and increased expression of glucose transporters (GLUT1, GLUT4), without changes in fatty acid transporters [89]. Il6 KO mice also exhibit shorter swim durations compared to WT mice [89]. IL-6 has been found to regulate glucose and fatty acid uptake through the upregulation of AMPK, an important regulator of fatty acid oxidation [89]. Decreased AMPK activation in Il6 KO mice during exercise leads to reduced fatty acid flux and oxidation, resulting in increased expression of Glut4 and increased glucose utilization [89]. Additional studies on Il6 KO mice have demonstrated impaired exercise capacity at high velocities and significantly lower plasma lactate levels after exercise, indicating impaired anaerobic glycolysis and increased glycogen depletion [90]. Muscle-specific Il6 KO mice also exhibit higher RER levels during exercise, indicating a preference for carbohydrate use over lipid use, which is accompanied by increased pyruvate dehydrogenase (PDH) activity [91]. These muscle-specific Il6 KO mice also had lower liver glucose level than WT mice during prolonged exercise, which may explain the higher RER and increased PDH activity, and indicates that skeletal muscle IL-6 may indirectly stimulate hepatic glucose production during exercise [92]. Administration of IL-6 recombinant to mice has been shown to increase exercise endurance and the expression of genes involved in oxidative phosphorylation, including pyruvate dehydrogenase kinase isozyme 4, which inhibits PDH activity [87]. Human studies have supported these findings by showing that injection of IL-6 recombinant into skeletal muscle increases systemic fatty acid oxidation [93]. Together, these studies indicate that IL-6 plays a critical role in balancing the utilization of fatty acids and glycogen during endurance exercise.

4. Conclusions

The regulation of fuel utilization in skeletal muscle is a complex interplay of multiple mechanisms, encompassing substrate bioavailability, transport, mitochondrial fuel utilization, transcriptional control, extracellular signaling, and metabolic shifts between glucose and lipid metabolism. This intricacy underscores the multifaceted nature of fuel utilization regulation. Furthermore, it is crucial to acknowledge that fuel utilization within skeletal muscle is not isolated but instead interacts with other tissues and organ systems, such as the liver and adipose tissue.
Moreover, understanding fuel utilization during exercise requires consideration of the broader context. Factors like pre-exercise metabolism influenced by nutrition and post-exercise factors like exercise type, intensity, duration, and environmental conditions all play integral roles and must be examined for a holistic understanding. Additionally, investigating the impact of fiber type heterogeneity, sex, and factors like menstrual cycles on metabolic rate and energy substrate partitioning is essential. These variables reflect the complexity of exercise metabolism.
Skeletal muscle, a major contributor to metabolic rate and energy utilization, assumes a central role in glycemic control, impacting glucose homeostasis under both insulin-stimulated and independent conditions. During exercise, skeletal muscle dynamically adjusts energy production, blood flow, and substrate utilization, influenced by factors like exercise intensity, duration, and hormonal responses, affecting the balance between carbohydrates and lipids as energy sources. After exercise, there is a significant shift toward lipid oxidation during the recovery period, vital for muscle glycogen replenishment. Understanding these metabolic intricacies is crucial for comprehending short- and long-term responses to exercise.
Overall, the metabolic conditions of the whole organism and the interactions between different tissues significantly shape fuel utilization in skeletal muscle. The differences between muscle-specific and whole-body knockout studies underscore the importance of the interplay between different tissues in regulating fuel utilization. To achieve a comprehensive understanding, future research should delve into the specific functions of various factors and mechanisms in a tissue-specific manner while considering interactions between tissues. This deeper understanding of fuel utilization can provide valuable insights into how exercise and skeletal muscle contribute to human health and overall quality of life. A summary of the results are presented in Table 1.

Author Contributions

A.P., S.D.V. and S.K. wrote the manuscript. All authors have read and agreed to the published version of the manuscript.

Funding

This work was funded by R01 DK116008 (NIDDK) to S.K.

Institutional Review Board Statement

Not applicable.

Informed Consent Statement

Not applicable.

Data Availability Statement

No new data were created or analyzed in this study. Data sharing is not applicable to this article.

Conflicts of Interest

The authors declare no conflict of interest.

References

  1. Roberts, C.K.; Barnard, R.J. Effects of exercise and diet on chronic disease. J. Appl. Physiol. 2005, 98, 3–30. [Google Scholar] [CrossRef] [PubMed]
  2. Egan, B.; Zierath, J.R. Exercise Metabolism and the Molecular Regulation of Skeletal Muscle Adaptation. Cell Metab. 2013, 17, 162–184. [Google Scholar] [CrossRef] [PubMed]
  3. Hughes, D.C.; Ellefsen, S.; Baar, K. Adaptations to Endurance and Strength Training. Cold Spring Harb. Perspect. Med. 2018, 8, a029769. [Google Scholar] [CrossRef] [PubMed]
  4. Booth, F.W.; Thomason, D.B. Molecular and cellular adaptation of muscle in response to exercise: Perspectives of various models. Physiol. Rev. 1991, 71, 541–585. [Google Scholar] [CrossRef]
  5. Sigal, R.J.; Kenny, G.P.; Boulé, N.G.; Wells, G.A.; Prud’homme, D.; Fortier, M.; Reid, R.D.; Tulloch, H.; Coyle, D.; Phillips, P.; et al. Effects of Aerobic Training, Resistance Training, or Both on Glycemic Control in Type 2 Diabetes. Ann. Intern. Med. 2007, 147, 357–369. [Google Scholar] [CrossRef] [PubMed]
  6. Burd, N.A.; West, D.W.D.; Moore, D.R.; Atherton, P.J.; Staples, A.W.; Prior, T.; Tang, J.E.; Rennie, M.J.; Baker, S.K.; Phillips, S.M. Enhanced Amino Acid Sensitivity of Myofibrillar Protein Synthesis Persists for up to 24 h after Resistance Exercise in Young Men1–3. J. Nutr. 2011, 141, 568–573. [Google Scholar] [CrossRef]
  7. Sjøberg, K.A.; Frøsig, C.; Kjøbsted, R.; Sylow, L.; Kleinert, M.; Betik, A.C.; Shaw, C.S.; Kiens, B.; Wojtaszewski, J.F.P.; Rattigan, S.; et al. Exercise Increases Human Skeletal Muscle Insulin Sensitivity via Coordinated Increases in Microvascular Perfusion and Molecular Signaling. Diabetes 2017, 66, 1501–1510. [Google Scholar] [CrossRef]
  8. Robinson, M.M.; Dasari, S.; Konopka, A.R.; Johnson, M.L.; Manjunatha, S.; Esponda, R.R.; Carter, R.E.; Lanza, I.R.; Nair, K.S. Enhanced Protein Translation Underlies Improved Metabolic and Physical Adaptations to Different Exercise Training Modes in Young and Old Humans. Cell Metab. 2017, 25, 581–592. [Google Scholar] [CrossRef]
  9. Chapman, M.A.; Arif, M.; Emanuelsson, E.B.; Reitzner, S.M.; Lindholm, M.E.; Mardinoglu, A.; Sundberg, C.J. Skeletal Muscle Transcriptomic Comparison between Long-Term Trained and Untrained Men and Women. Cell Rep. 2020, 31, 107808. [Google Scholar] [CrossRef]
  10. Smith, J.A.B.; Murach, K.A.; Dyar, K.A.; Zierath, J.R. Exercise metabolism and adaptation in skeletal muscle. Nat. Rev. Mol. Cell Biol. 2023, 24, 607–632. [Google Scholar] [CrossRef]
  11. Kelley, D.E.; Goodpaster, B.; Wing, R.R.; Simoneau, J.-A. Skeletal muscle fatty acid metabolism in association with insulin resistance, obesity, and weight loss. Am. J. Physiol.-Endocrinol. Metab. 1999, 277, E1130–E1141. [Google Scholar] [CrossRef]
  12. Kelley, D.E.; Mandarino, L.J. Fuel selection in human skeletal muscle in insulin resistance: A reexamination. Diabetes 2000, 49, 677–683. [Google Scholar] [CrossRef]
  13. Maunder, E.; Rothschild, J.A.; Fritzen, A.M.; Jordy, A.B.; Kiens, B.; Brick, M.J.; Leigh, W.B.; Chang, W.-L.; Kilding, A.E. Skeletal muscle proteins involved in fatty acid transport influence fatty acid oxidation rates observed during exercise. Pflug. Arch.-Eur. J. Physiol. 2023, 475, 1061–1072. [Google Scholar] [CrossRef] [PubMed]
  14. Manio, M.C.C.; Matsumura, S.; Masuda, D.; Inoue, K. CD36 is essential for endurance improvement, changes in whole-body metabolism, and efficient PPAR-related transcriptional responses in the muscle with exercise training. Physiol. Rep. 2017, 5, e13282. [Google Scholar] [CrossRef]
  15. McFarlan, J.T.; Yoshida, Y.; Jain, S.S.; Han, X.-X.; Snook, L.A.; Lally, J.; Smith, B.K.; Glatz, J.F.C.; Luiken, J.J.F.P.; Sayer, R.A.; et al. In Vivo, Fatty Acid Translocase (CD36) Critically Regulates Skeletal Muscle Fuel Selection, Exercise Performance, and Training-induced Adaptation of Fatty Acid Oxidation. J. Biol. Chem. 2012, 287, 23502–23516. [Google Scholar] [CrossRef] [PubMed]
  16. Iso, T.; Maeda, K.; Hanaoka, H.; Suga, T.; Goto, K.; Syamsunarno, M.R.A.A.; Hishiki, T.; Nagahata, Y.; Matsui, H.; Araia, M.; et al. Capillary Endothelial Fatty Acid Binding Proteins 4 and 5 Play a Critical Role in Fatty Acid Uptake in Heart and Skeletal Muscle. Arterioscler. Thromb. Vasc. Biol. 2013, 33, 2549–2557. [Google Scholar] [CrossRef]
  17. Iso, T.; Haruyama, H.; Sunaga, H.; Matsui, M.; Matsui, H.; Tanaka, R.; Umbarawan, Y.; Syamsunarno, M.R.A.A.; Yokoyama, T.; Kurabayashi, M.; et al. Exercise endurance capacity is markedly reduced due to impaired energy homeostasis during prolonged fasting in FABP4/5 deficient mice. BMC Physiol. 2019, 19, 1. [Google Scholar] [CrossRef]
  18. Romijn, J.A.; Coyle, E.F.; Sidossis, L.S.; Gastaldelli, A.; Horowitz, J.F.; Endert, E.; Wolfe, R.R. Regulation of endogenous fat and carbohydrate metabolism in relation to exercise intensity and duration. Am. J. Physiol.-Endocrinol. Metab. 1993, 265, E380–E391. [Google Scholar] [CrossRef] [PubMed]
  19. Huijsman, E.; van de Par, C.; Economou, C.; van der Poel, C.; Lynch, G.S.; Shoiswhohl, G.; Haemmerle, G.; Zechner, R.; Watt, M.J. Adipose triacylglycerol lipase deletion alters whole body energy metabolism and impairs exercise performance in mice. Am. J. Physiol.-Endocrinol. Metab. 2009, 297, E505–E513. [Google Scholar] [CrossRef] [PubMed]
  20. Fernandez, C.; Hansson, O.; Nevsten, P.; Holm, C.; Klint, C. Hormone-sensitive lipase is necessary for normal mobilization of lipids during submaximal exercise. Am. J. Physiol.-Endocrinol. Metab. 2008, 295, E179–E186. [Google Scholar] [CrossRef]
  21. Goa, K.L.; Brogden, R.N. l-Carnitine. Drugs 1987, 34, 1–24. [Google Scholar] [CrossRef] [PubMed]
  22. Fielding, R.; Riede, L.; Lugo, J.P.; Bellamine, A. l-Carnitine Supplementation in Recovery after Exercise. Nutrients 2018, 10, 349. [Google Scholar] [CrossRef]
  23. Kim, J.H.; Pan, J.H.; Lee, E.S.; Kim, Y.J. l-Carnitine enhances exercise endurance capacity by promoting muscle oxidative metabolism in mice. Biochem. Biophys. Res. Commun. 2015, 464, 568–573. [Google Scholar] [CrossRef] [PubMed]
  24. Herold, J.; Kalucka, J. Angiogenesis in Adipose Tissue: The Interplay between Adipose and Endothelial Cells. Front. Physiol. 2021, 11, 624903. [Google Scholar] [CrossRef]
  25. Zachwieja, N.J.; O’Connell, G.C.; Stricker, J.C.; Allen, J.; Vona-Davis, L.; Bryner, R.; Mandler, W.; Olfert, I.M. Loss of Adipocyte VEGF Impairs Endurance Exercise Capacity in Mice. Med. Sci. Sports Exerc. 2015, 47, 2329–2339. [Google Scholar] [CrossRef]
  26. Huertas, J.R.; Casuso, R.A.; Agustín, P.H.; Cogliati, S. Stay Fit, Stay Young: Mitochondria in Movement: The Role of Exercise in the New Mitochondrial Paradigm. Oxid. Med. Cell. Longev. 2019, 2019, 7058350. [Google Scholar] [CrossRef] [PubMed]
  27. Sorriento, D.; Di Vaia, E.; Iaccarino, G. Physical Exercise: A Novel Tool to Protect Mitochondrial Health. Front. Physiol. 2021, 12, 660068. [Google Scholar] [CrossRef]
  28. Zhang, L.; He, Z.; Zhang, Q.; Wu, Y.; Yang, X.; Niu, W.; Hu, Y.; Jia, J. Exercise Pretreatment Promotes Mitochondrial Dynamic Protein OPA1 Expression after Cerebral Ischemia in Rats. Int. J. Mol. Sci. 2014, 15, 4453–4463. [Google Scholar] [CrossRef]
  29. Rahn, J.J.; Stackley, K.D.; Chan, S.S.L. Opa1 Is Required for Proper Mitochondrial Metabolism in Early Development. PLoS ONE 2013, 8, e59218. [Google Scholar] [CrossRef]
  30. Caffin, F.; Prola, A.; Piquereau, J.; Novotova, M.; David, D.; Garnier, A.; Fortin, D.; Alavi, M.; Veksler, V.; Ventura-Clapier, R.; et al. Altered skeletal muscle mitochondrial biogenesis but improved endurance capacity in trained OPA1-deficient mice. J. Physiol. 2013, 591, 6017–6037. [Google Scholar] [CrossRef]
  31. Kitaoka, Y. The Role of Nrf2 in Skeletal Muscle on Exercise Capacity. Antioxidants 2021, 10, 1712. [Google Scholar] [CrossRef] [PubMed]
  32. Onoki, T.; Izumi, Y.; Takahashi, M.; Murakami, S.; Matsumaru, D.; Ohta, N.; Wati, S.M.; Hatanaka, N.; Katsuoka, F.; Okutsu, M.; et al. Skeletal muscle-specific Keap1 disruption modulates fatty acid utilization and enhances exercise capacity in female mice. Redox Biol. 2021, 43, 101966. [Google Scholar] [CrossRef] [PubMed]
  33. Oh, S.; Komine, S.; Warabi, E.; Akiyama, K.; Ishii, A.; Ishige, K.; Mizokami, Y.; Kuga, K.; Horie, M.; Miwa, Y.; et al. Nuclear factor (erythroid derived 2)-like 2 activation increases exercise endurance capacity via redox modulation in skeletal muscles. Sci. Rep. 2017, 7, 12902. [Google Scholar] [CrossRef] [PubMed]
  34. Bouviere, J.; Fortunato, R.S.; Dupuy, C.; Werneck-de-Castro, J.P.; Carvalho, D.P.; Louzada, R.A. Exercise-Stimulated ROS Sensitive Signaling Pathways in Skeletal Muscle. Antioxidants 2021, 10, 537. [Google Scholar] [CrossRef] [PubMed]
  35. Lin, J.; Wu, P.-H.; Tarr, P.T.; Lindenberg, K.S.; St-Pierre, J.; Zhang, C.; Mootha, V.K.; Jäger, S.; Vianna, C.R.; Reznick, R.M.; et al. Defects in Adaptive Energy Metabolism with CNS-Linked Hyperactivity in PGC-1α Null Mice. Cell 2004, 119, 121–135. [Google Scholar] [CrossRef] [PubMed]
  36. Dillon, L.M.; Rebelo, A.P.; Moraes, C.T. The Role of PGC-1 Coactivators in Aging Skeletal Muscle and Heart. IUBMB Life 2012, 64, 231–241. [Google Scholar] [CrossRef]
  37. Leone, T.C.; Lehman, J.J.; Finck, B.N.; Schaeffer, P.J.; Wende, A.R.; Boudina, S.; Courtois, M.; Wozniak, D.F.; Sambandam, N.; Bernal-Mizrachi, C.; et al. PGC-1α Deficiency Causes Multi-System Energy Metabolic Derangements: Muscle Dysfunction, Abnormal Weight Control and Hepatic Steatosis. PLoS Biol. 2005, 3, e101. [Google Scholar] [CrossRef] [PubMed]
  38. Handschin, C.; Chin, S.; Li, P.; Liu, F.; Maratos-Flier, E.; LeBrasseur, N.K.; Yan, Z.; Spigelman, B.M. Skeletal Muscle Fiber-type Switching, Exercise Intolerance, and Myopathy in PGC-1α Muscle-specific Knock-out Animals *. J. Biol. Chem. 2007, 282, 30014–30021. [Google Scholar] [CrossRef]
  39. Lin, J.; Wu, H.; Tarr, P.T.; Zhang, C.-Y.; Wu, Z.; Boss, O.; Michael, L.F.; Puigserver, P.; Isotani, E.; Olson, E.N.; et al. Transcriptional co-activator PGC-1α drives the formation of slow-twitch muscle fibres. Nature 2002, 418, 797–801. [Google Scholar] [CrossRef]
  40. Bourdeau Julien, I.; Sephton, C.F.; Dutchak, P.A. Metabolic Networks Influencing Skeletal Muscle Fiber Composition. Front. Cell Dev. Biol. 2018, 6, 125. [Google Scholar] [CrossRef]
  41. Leick, L.; Wojtaszewski, J.F.P.; Johansen, S.T.; Kiilerich, K.; Comes, G.; Hellsten, Y.; Hidalgo, J.; Pilegaard, H. PGC-1α is not mandatory for exercise- and training-induced adaptive gene responses in mouse skeletal muscle. Am. J. Physiol.-Endocrinol. Metab. 2008, 294, E463–E474. [Google Scholar] [CrossRef] [PubMed]
  42. Rowe, G.C.; El-Khoury, R.; Patten, I.S.; Rustin, P.; Arany, Z. PGC-1α is Dispensable for Exercise-Induced Mitochondrial Biogenesis in Skeletal Muscle. PLoS ONE 2012, 7, e41817. [Google Scholar] [CrossRef]
  43. Pilegaard, H.; Saltin, B.; Neufer, P.D. Exercise induces transient transcriptional activation of the PGC-1α gene in human skeletal muscle. J. Physiol. 2003, 546, 851–858. [Google Scholar] [CrossRef]
  44. Mathai, A.S.; Bonen, A.; Benton, C.R.; Robinson, D.L.; Graham, T.E. Rapid exercise-induced changes in PGC-1α mRNA and protein in human skeletal muscle. J. Appl. Physiol. 2008, 105, 1098–1105. [Google Scholar] [CrossRef]
  45. Watt, M.J.; Southgate, R.J.; Holmes, A.G.; Febbraio, M.A. Suppression of plasma free fatty acids upregulates peroxisome proliferator-activated receptor (PPAR) α and δ and PPAR coactivator 1α in human skeletal muscle, but not lipid regulatory genes. J. Mol. Endocrinol. 2004, 33, 533–544. [Google Scholar] [CrossRef]
  46. Little, J.P.; Safdar, A.; Bishop, D.; Tarnopolsky, M.A.; Gibala, M.J. An acute bout of high-intensity interval training increases the nuclear abundance of PGC-1α and activates mitochondrial biogenesis in human skeletal muscle. Am. J. Physiol.-Regul. Integr. Comp. Physiol. 2011, 300, R1303–R1310. [Google Scholar] [CrossRef] [PubMed]
  47. Lenhare, L.; Crisol, B.M.; Silva, V.R.R.; Katashima, C.K.; Cordeiro, A.V.; Pereira, K.D.; Luchessi, A.D.; da Silva, A.S.R.; Cintra, D.E.; Moura, L.P.; et al. Physical exercise increases Sestrin 2 protein levels and induces autophagy in the skeletal muscle of old mice. Exp. Gerontol. 2017, 97, 17–21. [Google Scholar] [CrossRef]
  48. Liu, X.; Niu, Y.; Yuan, H.; Huang, J.; Fu, L. AMPK binds to Sestrins and mediates the effect of exercise to increase insulin-sensitivity through autophagy. Metabolism 2015, 64, 658–665. [Google Scholar] [CrossRef]
  49. Zeng, N.; D’Souza, R.F.; Figueiredo, V.C.; Markworth, J.F.; Roberts, L.A.; Peake, J.M.; Mitchell, C.J.; Cameron-Smith, D. Acute resistance exercise induces Sestrin2 phosphorylation and p62 dephosphorylation in human skeletal muscle. Physiol. Rep. 2017, 5, e13526. [Google Scholar] [CrossRef] [PubMed]
  50. Kim, M.; Sujkowski, A.; Namkoong, S.; Gu, B.; Cobb, T.; Kim, B.; Kowalsky, A.H.; Cho, C.-S.; Semple, I.; Ro, S.-H.; et al. Sestrins are evolutionarily conserved mediators of exercise benefits. Nat. Commun. 2020, 11, 190. [Google Scholar] [CrossRef] [PubMed]
  51. Haldane, J. Methods of Air Analysis; Charles Griffin & Company, Ltd.: London, UK, 1918. [Google Scholar]
  52. Hill, A.V. Muscular Activity and Carbohydrate Metabolism. Science 1924, 60, 505–514. [Google Scholar] [CrossRef]
  53. Phua, W.W.T.; Wong, M.X.Y.; Liao, Z.; Tan, N.S. An aPPARent Functional Consequence in Skeletal Muscle Physiology via Peroxisome Proliferator-Activated Receptors. Int. J. Mol. Sci. 2018, 19, 1425. [Google Scholar] [CrossRef]
  54. Muoio, D.M.; MacLean, P.S.; Lang, D.B.; Li, S.; Houmard, J.A.; Way, J.M.; Winegar, D.A.; Corton, J.C.; Dohm, G.L.; Kraus, W.E. Fatty Acid Homeostasis and Induction of Lipid Regulatory Genes in Skeletal Muscles of Peroxisome Proliferator-activated Receptor (PPAR) α Knock-out Mice: Evidence for compensatory regulation by pparδ. J. Biol. Chem. 2002, 277, 26089–26097. [Google Scholar] [CrossRef]
  55. Greene, N.P.; Fluckey, J.D.; Lambert, B.S.; Greene, E.S.; Riechman, S.E.; Crouse, S.F. Regulators of blood lipids and lipoproteins? PPARδ and AMPK, induced by exercise, are correlated with lipids and lipoproteins in overweight/obese men and women. Am. J. Physiol.-Endocrinol. Metab. 2012, 303, E1212–E1221. [Google Scholar] [CrossRef] [PubMed]
  56. Russell, A.P.; Feilchenfeldt, J.; Schreiber, S.; Praz, M.; Crettenand, A.; Gobelet, C.; Meier, C.A.; Bell, D.R.; Kralli, A.; Giacobino, J.-P.; et al. Endurance Training in Humans Leads to Fiber Type-Specific Increases in Levels of Peroxisome Proliferator-Activated Receptor-γ Coactivator-1 and Peroxisome Proliferator-Activated Receptor-α in Skeletal Muscle. Diabetes 2003, 52, 2874–2881. [Google Scholar] [CrossRef]
  57. Lee, W.J.; Kim, M.; Park, H.-S.; Kim, H.S.; Jeon, M.H.; Oh, K.S.; Koh, E.H.; Won, J.C.; Kim, M.-S.; Oh, G.T.; et al. AMPK activation increases fatty acid oxidation in skeletal muscle by activating PPARα and PGC-1. Biochem. Biophys. Res. Commun. 2006, 340, 291–295. [Google Scholar] [CrossRef] [PubMed]
  58. Finck, B.N.; Bernal-Mizrachi, C.; Han, D.H.; Coleman, T.; Sambandam, N.; LaRiviere, L.L.; Holloszy, J.O.; Semenkovich, C.F.; Kelly, D.P. A potential link between muscle peroxisome proliferator- activated receptor-α signaling and obesity-related diabetes. Cell Metab. 2005, 1, 133–144. [Google Scholar] [CrossRef] [PubMed]
  59. Fan, L.; Sweet, D.R.; Prosdocimo, D.A.; Vinayachandran, V.; Chan, E.R.; Zhang, R.; Ilkayeva, O.; Lu, Y.; Keerthy, K.S.; Booth, C.E.; et al. Muscle Krüppel-like factor 15 regulates lipid flux and systemic metabolic homeostasis. J. Clin. Investig. 2021, 131, e139496. [Google Scholar] [CrossRef]
  60. Haldar, S.M.; Jeyaraj, D.; Anand, P.; Zhu, H.; Lu, Y.; Prosdocimo, D.A.; Eapen, B.; Kawanami, D.; Okutsu, M.; Brotto, L.; et al. Kruppel-like factor 15 regulates skeletal muscle lipid flux and exercise adaptation. Proc. Natl. Acad. Sci. USA 2012, 109, 6739–6744. [Google Scholar] [CrossRef]
  61. Cortez-Toledo, O.; Schnair, C.; Sangngern, P.; Metzger, D.; Chao, L.C. Nur77 deletion impairs muscle growth during developmental myogenesis and muscle regeneration in mice. PLoS ONE 2017, 12, e0171268. [Google Scholar] [CrossRef]
  62. Chao, L.C.; Wroblewski, K.; Ilkayeva, O.R.; Stevens, R.D.; Bain, J.; Meyer, G.A.; Schenk, S.; Martinez, L.; Vergnes, L.; Narkar, V.A.; et al. Skeletal muscle Nur77 expression enhances oxidative metabolism and substrate utilization. J. Lipid Res. 2012, 53, 2610–2619. [Google Scholar] [CrossRef]
  63. Liu, H.-W.; Chang, S.-J. Moderate Exercise Suppresses NF-κB Signaling and Activates the SIRT1-AMPK-PGC1α Axis to Attenuate Muscle Loss in Diabetic db/db Mice. Front. Physiol. 2018, 9, 636. [Google Scholar] [CrossRef] [PubMed]
  64. Minegishi, Y.; Haramizu, S.; Misawa, K.; Shimotoyodome, A.; Hase, T.; Murase, T. Deletion of nuclear factor-κB p50 upregulates fatty acid utilization and contributes to an anti-obesity and high-endurance phenotype in mice. Am. J. Physiol.-Endocrinol. Metab. 2015, 309, E523–E533. [Google Scholar] [CrossRef]
  65. Gallego-Selles, A.; Galvan-Alvarez, V.; Martinez-Canton, M.; Garcia-Gonzalez, E.; Morales-Alamo, D.; Santana, A.; Gonzalez-Henriquez, J.J.; Dorado, C.; Calbet, J.A.L.; Martin-Rincon, M. Fast regulation of the NF-κB signalling pathway in human skeletal muscle revealed by high-intensity exercise and ischaemia at exhaustion: Role of oxygenation and metabolite accumulation. Redox Biol. 2022, 55, 102398. [Google Scholar] [CrossRef] [PubMed]
  66. Jiang, L.Q.; Franck, N.; Egan, B.; Sjögren, R.J.O.; Katayama, M.; Duque-Guimaraes, D.; Arner, P.; Zierath, J.R.; Krook, A. Autocrine role of interleukin-13 on skeletal muscle glucose metabolism in type 2 diabetic patients involves microRNA let-7. Am. J. Physiol.-Endocrinol. Metab. 2013, 305, E1359–E1366. [Google Scholar] [CrossRef]
  67. Knudsen, N.H.; Stanya, K.J.; Hyde, A.L.; Chalom, M.M.; Alexander, R.K.; Liou, Y.-H.; Starost, K.A.; Gangl, M.R.; Jacobi, D.; Liu, S.; et al. Interleukin 13 drives metabolic conditioning of muscle to endurance exercise. Science 2020, 368, eaat3987. [Google Scholar] [CrossRef]
  68. Young, P.A.; Senkal, C.E.; Suchanek, A.L.; Grevengoed, T.J.; Lin, D.D.; Zhao, L.; Crunk, A.E.; Klett, E.L.; Füllekrug, J.; Obeid, L.M.; et al. Long-chain acyl-CoA synthetase 1 interacts with key proteins that activate and direct fatty acids into niche hepatic pathways. J. Biol. Chem. 2018, 293, 16724–16740. [Google Scholar] [CrossRef] [PubMed]
  69. Li, L.O.; Grevengoed, T.J.; Paul, D.S.; Ilkayeva, O.; Koyes, T.R.; Pascual, F.; Newgard, C.B.; Muoio, D.M.; Coleman, R.A. Compartmentalized Acyl-CoA Metabolism in Skeletal Muscle Regulates Systemic Glucose Homeostasis. Diabetes 2015, 64, 23–35. [Google Scholar] [CrossRef] [PubMed]
  70. Fredriksson, J.; Anevski, D.; Almgren, P.; Sjögren, M.; Lyssenko, V.; Carlson, J.; Isomaa, B.; Taskinen, M.-R.; Groop, L.; Orho-Melander, M. Variation in GYS1 Interacts with Exercise and Gender to Predict Cardiovascular Mortality. PLoS ONE 2007, 2, e285. [Google Scholar] [CrossRef]
  71. Pederson, B.A.; Cope, C.R.; Schroeder, J.M.; Smith, M.W.; Irimia, J.M.; Thurberg, B.L.; DePaoli-Roach, A.A.; Roach, P.J. Exercise Capacity of Mice Genetically Lacking Muscle Glycogen Synthase: In mice, muscle glycogen is not essential for exercise. J. Biol. Chem. 2005, 280, 17260–17265. [Google Scholar] [CrossRef]
  72. Xirouchaki, C.E.; Mangiafico, S.P.; Bate, K.; Ruan, Z.; Huang, A.M.; Tedjosiswoyo, B.W.; Lamont, B.; Pong, W.; Favaloro, J.; Blair, A.R.; et al. Impaired glucose metabolism and exercise capacity with muscle-specific glycogen synthase 1 (gys1) deletion in adult mice. Mol. Metab. 2016, 5, 221–232. [Google Scholar] [CrossRef]
  73. Nguyen, H.P.; Yi, D.; Lin, F.; Viscarra, J.A.; Tabuchi, C.; Ngo, K.; Shin, G.; Lee, A.Y.; Wang, Y.; Sul, H.S. Aifm2, a NADH oxidase, supports robust glycolysis and is required for cold- and diet-induced thermogenesis. Mol. Cell 2020, 77, 600–617.e4. [Google Scholar] [CrossRef]
  74. Nguyen, H.P.; Villivalam, S.D.; Jung, B.C.; You, D.; Lin, F.; Yi, D.; Pi, A.; Ma, K.; Jung, S.; Park, S.-H.; et al. AIFM2 Is Required for High-Intensity Aerobic Exercise in Promoting Glucose Utilization. Diabetes 2022, 71, 2084–2093. [Google Scholar] [CrossRef] [PubMed]
  75. Binsch, C.; Jelenik, T.; Pfitzer, A.; Dille, M.; Müller-Lühlhoff, S.; Hartwig, S.; Karpinski, S.; Lehr, S.; Kabra, D.G.; Chadt, A.; et al. Absence of the kinase S6k1 mimics the effect of chronic endurance exercise on glucose tolerance and muscle oxidative stress. Mol. Metab. 2017, 6, 1443–1453. [Google Scholar] [CrossRef]
  76. Dutchak, P.A.; Estill-Terpack, S.J.; Plec, A.A.; Zhao, X.; Yang, C.; Chen, J.; Ko, B.; Deberardinis, R.J.; Yu, Y.; Tu, B.P. Loss of a Negative Regulator of mTORC1 Induces Aerobic Glycolysis and Altered Fiber Composition in Skeletal Muscle. Cell Rep. 2018, 23, 1907–1914. [Google Scholar] [CrossRef] [PubMed]
  77. Graber, T.G.; Fry, C.S.; Brightwell, C.R.; Moro, T.; Maroto, R.; Bhattarai, N.; Porter, C.; Wakamiya, M.; Rasmussen, B.B. Skeletal muscle–specific knockout of DEP domain containing 5 protein increases mTORC1 signaling, muscle cell hypertrophy, and mitochondrial respiration. J. Biol. Chem. 2019, 294, 4091–4102. [Google Scholar] [CrossRef]
  78. Cho, C.-S.; Kim, Y.; Park, S.-R.; Kim, B.; Davis, C.; Hwang, I.; Brooks, S.V.; Lee, J.H.; Kim, M. Simultaneous loss of TSC1 and DEPDC5 in skeletal and cardiac muscles produces early-onset myopathy and cardiac dysfunction associated with oxidative damage and SQSTM1/p62 accumulation. Autophagy 2021, 18, 2303–2322. [Google Scholar] [CrossRef] [PubMed]
  79. Mihaylova, M.M.; Shaw, R.J. The AMPK signalling pathway coordinates cell growth, autophagy and metabolism. Nat. Cell Biol. 2011, 13, 1016–1023. [Google Scholar] [CrossRef]
  80. O’Neill, H.M.; Maarbjerg, S.J.; Crane, J.D.; Jeppesen, J.; Jørgensen, S.B.; Schertzer, J.D.; Shyroka, O.; Kiens, B.; van Denderen, B.J.; Tarnopolsky, M.A.; et al. AMP-activated protein kinase (AMPK) β1β2 muscle null mice reveal an essential role for AMPK in maintaining mitochondrial content and glucose uptake during exercise. Proc. Natl. Acad. Sci. USA 2011, 108, 16092–16097. [Google Scholar] [CrossRef]
  81. Viollet, B. The Energy Sensor AMPK: Adaptations to Exercise, Nutritional and Hormonal Signals. In Hormones, Metabolism and the Benefits of Exercise; Spiegelman, B., Ed.; Springer: Berlin/Heidelberg, Germany, 2017. [Google Scholar]
  82. Fan, W.; Waizenegger, W.; Lin, C.S.; Sorrentino, V.; He, M.-X.; Wall, C.E.; Li, H.; Liddle, C.; Yu, R.T.; Atkins, A.R.; et al. PPARδ Promotes Running Endurance by Preserving Glucose. Cell Metab. 2017, 25, 1186–1193.e4. [Google Scholar] [CrossRef] [PubMed]
  83. Flynn, J.M.; Meadows, E.; Fiorotto, M.; Klein, W.H. Myogenin Regulates Exercise Capacity and Skeletal Muscle Metabolism in the Adult Mouse. PLoS ONE 2010, 5, e13535. [Google Scholar] [CrossRef] [PubMed]
  84. Ziello, J.E.; Jovin, I.S.; Huang, Y. Hypoxia-Inducible Factor (HIF)-1 Regulatory Pathway and its Potential for Therapeutic Intervention in Malignancy and Ischemia. Yale J. Biol. Med. 2007, 80, 51–60. [Google Scholar]
  85. Mason, S.D.; Howlett, R.A.; Kim, M.J.; Olfert, I.M.; Hogan, M.C.; McNulty, W.; Hickey, R.P.; Wagner, P.D.; Kahn, C.R.; Giordano, F.J.; et al. Loss of Skeletal Muscle HIF-1α Results in Altered Exercise Endurance. PLoS Biol. 2004, 2, e288. [Google Scholar] [CrossRef]
  86. Hui, S.; Ghergurovich, J.M.; Morscher, R.J.; Jang, C.; Teng, X.; Lu, W.; Esparza, L.A.; Reya, T.; Zhan, L.; Guo, J.Y.; et al. Glucose feeds the TCA cycle via circulating lactate. Nature 2017, 551, 115–118. [Google Scholar] [CrossRef]
  87. Leuchtmann, A.B.; Furrer, R.; Steurer, S.A.; Schneider-Heieck, K.; Karrer-Cardel, B.; Sagot, Y.; Handschin, C. Interleukin-6 potentiates endurance training adaptation and improves functional capacity in old mice. J. Cachexia Sarcopenia Muscle 2022, 13, 1164–1176. [Google Scholar] [CrossRef] [PubMed]
  88. Chow, L.S.; Gerszten, R.E.; Taylor, J.M.; Pedersen, B.K.; van Praag, H.; Trappe, S.; Febbraio, M.A.; Galis, Z.S.; Gao, Y.; Haus, J.M.; et al. Exerkines in health, resilience and disease. Nat. Rev. Endocrinol. 2022, 18, 273–289. [Google Scholar] [CrossRef]
  89. Łukaszuk, B.; Bialuk, I.; Górski, J.; Zajaczkiewicz, M.; Winnicka, M.M.; Chabowski, A. A Single Bout of Exercise Increases the Expression of Glucose but not Fatty Acid Transporters in Skeletal Muscle of IL-6 KO Mice. Lipids 2012, 47, 763–772. [Google Scholar] [CrossRef] [PubMed]
  90. Wojewoda, M.; Kmiecik, K.; Ventura-Clapier, R.; Fortin, D.; Onopiuk, M.; Jakubczyk, J.; Sitek, B.; Fedorowicz, A.; Majerczak, J.; Kaminski, K. Running Performance at High Running Velocities Is Impaired but V′O2max and Peripheral Endothelial Function Are Preserved in IL-6−/− Mice. PLoS ONE 2014, 9, e88333. [Google Scholar] [CrossRef] [PubMed]
  91. Gudiksen, A.; Schwartz, C.L.; Bertholdt, L.; Joensen, E.; Knudsen, J.G.; Pilegaard, H. Lack of Skeletal Muscle IL-6 Affects Pyruvate Dehydrogenase Activity at Rest and during Prolonged Exercise. PLoS ONE 2016, 11, e0156460. [Google Scholar] [CrossRef] [PubMed]
  92. Bertholdt, L.; Gudiksen, A.; Schwartz, C.L.; Knudsen, J.G.; Pilegaard, H. Lack of skeletal muscle IL-6 influences hepatic glucose metabolism in mice during prolonged exercise. Am. J. Physiol.-Regul. Integr. Comp. Physiol. 2017, 312, R626–R636. [Google Scholar] [CrossRef] [PubMed]
  93. Wolsk, E.; Mygind, H.; Grøndahl, T.S.; Pedersen, B.K.; van Hall, G. IL-6 selectively stimulates fat metabolism in human skeletal muscle. Am. J. Physiol.-Endocrinol. Metab. 2010, 299, E832–E840. [Google Scholar] [CrossRef] [PubMed]
Table 1. Summary of Factors Affecting Fuel Utilization in Skeletal Muscle During Exercise.
Table 1. Summary of Factors Affecting Fuel Utilization in Skeletal Muscle During Exercise.
Gene/Protein Genetic ManipulationAssociated FunctionExercise PhenotypeEffects on Fuel UtilizationReferences
CD36Whole-body KOFatty acid transporterPromote endurance exercise capacityPromote fatty acid transport into muscle, allowing for metabolic switching[14]
ATGLWhole-body KOTriacylglycerol lipasePromote endurance exercise capacityPromote exercise-stimulated lipolysis[19]
HSLWhole-body KOTriacylglycerol lipasePromote endurance exercise capacityPromote exercise-stimulated lipolysis[20]
L-CarnitineOverexpression
(oral dose administered)		Cofactor for fatty acid transformation and transportEnhance endurance exercise capacityPromote fat utilization and mitochondrial biogenesis[23]
VEGFAdipocyte-specific KOPromotes angiogenesisPromote exercise toleranceIncrease adipose capillarity, increasing bioavailability of free fatty acids[25]
OPA1HaplodeficiencyRegulate mitochondrial fusionNot sufficient to affect exercise capacity by itselfPromote fatty acid oxidation[30]
NRF2Whole-body KORegulate genes in oxidative stress responsePromote endurance exercise capacityPromote fatty acid oxidation[33,34]
KEAP1Muscle-specific KONegatively regulates NRF2Decrease endurance and resistance exercise capacityDecreases fatty acid oxidation[32]
PGC-1aWhole-body KO, Muscle-specific KOCotranscription factor that regulates fatty acid oxidation, mitochondrial biogenesis, and mitochondrial functionPromote exercise tolerance and slow-twitch muscle fiber contentMaintain glucose homeostasis, promote fatty acid oxidation[35,37,38,39]
SestrinsWhole-body KOStress-induced protein, activates downstream pathways to regulate metabolismPromote endurance exercise capacityMaintain glucose homeostasis, promote fatty acid oxidation[50]
PPARαWhole-body KO, muscle-specific overexpressionTranscription factor that regulates lipid and glucose homeostasisPromote endurance exercise capacityFavor lipid utilization over glucose, promotes fatty acid oxidation[54,57,58]
KLF15Whole-body KOTranscription factor that regulates many metabolic processesPromote endurance exercise capacityAllows metabolic switching; promotes fatty acid oxidation in endurance exercise[60]
NR4A1 or NUR77Muscle-specific overexpressionTranscription factor that affects muscle fiber content Increase muscle contractile functionPromotes fatty acid oxidation over glucose oxidation[62]
P50 (NF-κB)Whole-body KOTranscription factor that regulates inflammation and infectionDecrease endurance exercise capacityDecreases fatty acid oxidation and promotes glucose oxidation[64]
Il-13Whole-body KOAnti-inflammatory cytokinePromote exercise capacityPromote fatty acid oxidation and mitochondrial biogenesis[67]
ACSL1Muscle-specific KODirects fatty acids into mitochondria for fatty acid oxidationPromote endurance exercise capacityPromotes fatty acid oxidation over glucose use[69]
GYSMuscle-specific KOKey enzyme in synthesis of glycogen in skeletal musclePromote endurance exercise capacityMaintains muscle glycogen for use as a fuel source[72]
AIFM2Muscle targeted KD and OE, muscle-specific haploinsufficiency (ACTA-Cre)NADH oxidoreductasePromote high-intensity exercisePromote glucose utilization over lipid use[74]
S6K1Whole-body KOComponent of mTORC signaling pathway that controls cell growthDecrease exercise capacityDownregulate ketogenesis, and promote glucose utilization over fatty acid oxidation[75]
mTORC1Muscle-specific activation (via KO of negative regulators)Regulator of protein translation and cellular metabolismMuscle hypertrophy; no observed differences in exercise capacityIncrease glycolytic fibers in muscle, promoting glucose utilization[76,77,78]
AMPKWhole-body KOWhole-body stress sensing kinase that regulates energy metabolismPromote exercise capacityPromote mitochondrial content and glucose uptake[80]
PPARδMuscle-specific overexpressionNuclear receptor that is a key regulator of fatty acid metabolism in musclePromote endurance exercise capacityStimulate fatty acid oxidation and suppress glucose utilization[82]
MyogeninWhole-body KORegulates skeletal muscle development during embryonic and fetal stagesDecrease exercise capacityIncrease sensitivity to depletion of glycogen reserves; decreased efficiency of fatty acid and glucose use[83]
HIF-1αMuscle-specific KOProtein complex that responds to low oxygen conditions (hypoxia)Decrease exercise capacity; prevent muscle damage from repeated exercisePromotes glucose utilization over fatty acid oxidation[85]
Il-6Whole-body KO, muscle-specific KO, whole-body OE (injection), muscle-specific OE (injection)Myokine believed to be largely anti-inflammatoryIncrease exercise capacityIncrease fatty acid oxidation[87,89,90,93]
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Pi, A.; Villivalam, S.D.; Kang, S. The Molecular Mechanisms of Fuel Utilization during Exercise. Biology 2023, 12, 1450. https://doi.org/10.3390/biology12111450

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Pi A, Villivalam SD, Kang S. The Molecular Mechanisms of Fuel Utilization during Exercise. Biology. 2023; 12(11):1450. https://doi.org/10.3390/biology12111450

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Pi, Anna, Sneha Damal Villivalam, and Sona Kang. 2023. "The Molecular Mechanisms of Fuel Utilization during Exercise" Biology 12, no. 11: 1450. https://doi.org/10.3390/biology12111450

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Pi, A., Villivalam, S. D., & Kang, S. (2023). The Molecular Mechanisms of Fuel Utilization during Exercise. Biology, 12(11), 1450. https://doi.org/10.3390/biology12111450

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