We have previously reported that dietary ketogenic amino acids (KAAs) modulate hepatic de novo lipogenesis (DNL) and prevent hepatic steatosis in mice. However, the dependence of the metabolic phenotypes generated by KAA on the type of dietary lipid source remains unclear.
The aim of this study was to assess the effect of KAA combined with different dietary lipid sources on hepatic DNL and tissue lipid partitioning in mice.
We compared three different KAA-supplemented diets, in which a portion of the dietary protein was replaced by five major essential amino acids (Leu, Ile, Val, Lys and Thr) in high-fat diets based on palm oil (PO), high-oleic safflower oil (FO) or soy oil (SO). To compare the effects of these diets in C57B6 mice, the differential regulation of DNL and dietary lipid partitioning due to KAA was assessed using stable isotopic flux analysis.
The different dietary oils showed strikingly different patterns of lipid partitioning and accumulation in tissues. High-PO diets increased both hepatic and adipose triglycerides (TG), whereas high-FO and high-SO diets increased hepatic and adipose TG, respectively. Stable isotopic flux analysis revealed high rates of hepatic DNL in high-PO and high-FO diets, whereas it was reduced in the high-SO diet. KAA supplementation in high-PO and high-FO diets reduced hepatic TG by reducing the DNL of palmitate and the accumulation of dietary oleate. However, KAA supplementation in the high-SO diet failed to reduce hepatic DNL and TG. Interestingly, KAA reduced SO-induced accumulation of hepatic linoleate and enhanced SO-induced accumulation of dietary oleate.
Overall, the reduction of hepatic TG by KAA is dependent on dietary lipid sources and occurs through the modulation of DNL and altered partitioning of dietary lipids. The current results provide further insight into the underlying mechanisms of hepatic lipid reduction by amino acids.
The rising prevalence of obesity—a major health concern worldwide—has been linked to a number of cardiovascular and metabolic disorders, such as hypertension, insulin resistance, hyperlipidemia and, more recently, non-alcoholic fatty liver disease, also known as hepatic steatosis.1, 2 Physical inactivity, dietary behavior and inherited predisposition are the predominant causes of excessive fat accumulation in adipose and non-adipose tissues, which subsequently leads to metabolic disorders. In diets designed to prevent and treat such excessive fat accumulation by manipulating energy content, macronutrient distribution has been examined by controlling the proportions of fat, carbohydrate and protein, commonly with reductions in dietary fat.3, 4 Although this approach appears to be effective for reducing energy density and increasing the loss of lipids in adipose tissue in the short term,3, 4 increased dietary carbohydrate levels activate de novo lipogenesis (DNL) to compensate for the lower fat intake and then induce lipid accumulation in non-adipose tissues in the long term.5, 6 Likewise, a low-carbohydrate diet has been shown to be an effective approach for body fat reduction in the short term, but the long-term effects have not been established.7 Recent studies in humans show that a high-protein diet may also have beneficial effects on body fat maintenance by inducing satiety or reducing hepatic lipid deposition.8
In addition to macronutrient proportions, specific macronutrient elements such as sugars,9 fatty acids10 and amino acids11, 12 are important factors in the regulation and dysregulation of lipid metabolism. For example, the difference between monounsaturated fatty acids (MUFAs) and saturated fatty acids (SFAs) has been well characterized;13, 14, 15 these two types of fatty acid affect postprandial lipid metabolism differently.16, 17 In addition, polyunsaturated fatty acid (PUFA) supplementation has been reported to prevent insulin resistance18, 19 and hepatic steatosis.20, 21 Several reports suggest that dietary medium-chain fatty acids promote energy expenditure and fatty acid oxidation and improve lipid metabolism in rats22 and humans23 compared with long-chain fatty acids.
Previous studies have shown that dietary withdrawal of the essential amino acids lysine or threonine induces severe hepatic steatosis in rodents.11, 12 Furthermore, a role for the amino-acid deprivation sensor GCN2 in regulating hepatic lipid homeostasis has recently been revealed.24, 25 Leucine and lysine, which are both ketogenic amino acids (KAAs), have unique metabolic characteristics and produce various short-chain fatty acyl-CoAs, such as isovalaryl-CoA, 3-hydroxy-3-methylglutaryl-CoA and glutaryl-CoA, through catabolism. In addition to leucine and lysine, isoleucine, valine and threonine also produce short, branched-chain acyl-CoAs.26 A few studies have reported the potential importance of these branched-chain acyl-CoAs in regulating lipid homeostasis through transcription factors or nuclear receptors.27, 28 We previously reported that the supplementation of KAA that generate acyl-CoA rescued palmitate-induced hepatic lipoapoptosis in vitro29 and also prevented hepatic steatosis through the repression of DNL in mice.30 However, the underlying mechanisms and effects of KAA versus dietary lipid species on these phenotypes have yet to be elucidated.
In this study, we examined KAA supplementation in C57B6 mice fed either a regular high-lard diet or one of three different high-fat diets (HFDs), that is, SFA-rich palm oil (PO), MUFA-rich high-oleic safflower oil (FO) and PUFA-rich soy oil (SO) diets. Using gas chromatography–mass spectrometry (GC-MS)-based lipid profiling and stable isotopic metabolic flux analysis, we assessed the dependence of the effect of KAA on the type of dietary lipid in terms of both the regulation of hepatic DNL and the dietary lipid partitioning to tissues.
Materials and methods
All studies were reviewed and approved by the Animal Care Committee of Ajinomoto Co. Inc. Ten-week-old male C57B6 mice and ob/ob mice, were obtained from Charles River Laboratory, Japan Inc. (Yokohama, Japan). All mice were housed in colony cages and maintained on a 12:12-h light and dark rhythm with free access to water. After 3 h of fasting, blood was collected on ice in tubes containing EDTA (NONCLOT-D, Daiichi Pure Chemicals, Tokyo, Japan). Liver, epididimal fat and gastrocnemius muscle samples were collected for lipid and gene expression analysis. All collected tissues were snap-frozen in liquid nitrogen and stored at −80 °C.
As documented in our previous report, we manipulated dietary amino-acid composition by replacing part of the protein content with a free amino-acid mixture in either a control diet or a high-KAA diet.30 Supplementary Tables S1 and S2 show the composition of the diets used in this study. The casein-mimic-free amino-acid mixture used for the control diet contained the following components: 2.5% His, 4.5% Phe, 8.8% Lys-HCl, 1.1% Trp, 3.8% Thr, 2.4% Thr, 2.4% Met, 4.5% Ile, 5.7% Val, 8.1% Leu, 9.4% Pro, 9.4% Asn H2O, 4.9% Tyr, 2.6% Ala, 3.3% Arg, 5.1% Ser, 9.2% Glu, 9.2% Gln, 1.6% Gly, 0.5% cysteine, 3.2% Asp and 6.2% starch. On the basis of the partial protein replacement by free KAA, the essential amino acid/non-essential amino acid ratio in the diet was fortified from the control value of 0.8 (for casein) to 1.76. To avoid differences in the amounts of dietary total amino acids, fat and carbohydrates among the diets, the total amino acids, including protein–amino acids, were equalized, if necessary, using casein-mimic-free amino-acid mixture to provide 20% of dietary calories. On the basis of this protocol, we prepared the high-lard diet and the three different types of HFDs consisting of PO, FO and SO. As a percentage of total energy, the diets consisted of 26.4% carbohydrate, 52.6% fat and 20% protein plus amino acids. The high-KAA diet contained 13.1% basal casein, with 6.9% consisting of a selected KAA mixture of leucine, isoleucine, valine, lysine and threonine in the proportions shown in Supplementary Tables S1 and S2.
Blood glucose, cholesterol and triglycerides (TG) were measured using DRI-CHEM5500 (Fujifilm, Tokyo, Japan). Plasma-free fatty acids were determined using an enzymatic method with an automated kit according to the manufacturer's specifications (Wako Pure Chemical Industries, Osaka, Japan). Serum leptin and insulin were determined using commercial mouse ELISA kits (Seikagaku-kogyo Co., Tokyo, Japan).
The energy expenditure of individual mice was measured using indirect calorimetry. An animal was housed in a metabolic cage for 24 h, allowing for the separate collection of urine and feces.28 Food was available between 1900 and 0800 hours. Oxygen consumption and CO2 production were determined every 5 min in an open chamber with the mass spectrometry-based O2 and CO2 analyzer ARCO-2000 (ARCO system, Chiba, Japan). Oxygen consumption was normalized by lean body mass.
Tissue lipid extraction
Liver lipid extraction was performed using isopropanol and hexane based on a modification of a method described previously.31 This procedure extracts a mixture of TG, diglycerides, mono-glycerides, cholesterol, fatty acids and other polar lipids. After extraction, fractionation was performed to collect each lipid class. In brief, 150 mg of liver or 40 mg of epididymal fat tissue was homogenized in 1.5 ml of isopropanol and then sonicated for 30 min after the addition of 3 ml hexane. As an internal standard, 0.1 mg triheptadecanoic acid was added to each sample. The homogenate was incubated overnight for further extraction. After the addition of 1 ml saline, the mixture was centrifuged at 3500 r.p.m. for 15 min, and the supernatant was collected into new tubes.
Because the extracted solvent contains a mixture of different classes of lipids, fractionation was performed to efficiently analyze each class of lipids using a silica gel column together with gradual elution with solvents of increasing polarity as described in a previous report.32 The extracted solvent was evaporated to dryness, resolved in 500 μl of isooctane/ethyl acetate (10:1) and applied to a preequiberated silica gel column (InertSep SI, GL Sciences, Tokyo, Japan). The column was then eluted with 4 ml isooctane/ethyl acetate (10:1). This fraction contained cholesterol esters and TG. This process was repeated with isooctane/ethyl acetate (3:1) and methanol, and each elutant contained free fatty acids, diglycerides and polar lipids.
Lipid analysis by GC-MS
To analyze the fatty acid profile of TG, the triglyceride fraction was saponified with 0.5 N NaOH dissolved in methanol, and methyl was esterized with boron trifluoride as described previously.29 The fatty acid methyl esters were analyzed using electron impact ionization by GC-MS on an Agilent 5975C model coupled with a 7890A model gas chromatograph (Agilent, Santa Clara, CA, USA). A DB-225 ms capillary column (30 m × 0.25 mm film 0.25 μm, Agilent) was used in all lipid analyses. The initial oven temperature was 190 °C, which was then increased by 3 °C min−1 to 230 °C and held for 2 min. The Mass Selective Detector (MSD) transfer line was set at 280 °C. The components of the sample were repetitively scanned from 50 to 550 m/z. The MS quad was 150 °C, and the MS source was set at 230 °C.
Peak enumeration and spectral deconvolution was performed by AMDIS software (http://chemdata.nist.gov/mass-spc/amdis/; National Institute of Standards and Technology). The resulting ELU files (output from AMDIS) were further analyzed by SpectConnect software (http://spectconnect.mit.edu/) to identify well-conserved peaks among multiple GC-MS chromatograms.33
Lipogenic flux estimation
Two weeks before killing, mice were given an intraperitoneal injection of deuterated water (D2O) equal to 4% of their body weight in saline at 1000 hours. Animals were then maintained on drinking water containing 6% D2O for 2 weeks. This procedure was designed to maintain deuterium enrichment in the body water at around 3–4% throughout the study. Animals were fasted for 3 h before killing.
Using D2O and mass isotopomer analysis, the rates of synthesis can be calculated from the ratio of isotope-labeled fatty acids to unlabeled fatty acids.34, 35 The major peaks in the ion chromatogram of fatty acids in the liver are the long-chain fatty acids palmitate (16:0), stearate (18:0) and oleate (18:1). The fractional synthesis rates of these three fatty acids were calculated. The chain elongation flux of palmitate to stearate was determined by dividing the amount of newly synthesized C18:0 by that of newly synthesized 16:0. The desaturation flux of stearate to oleate was calculated by dividing the amount of newly synthesized 18:1 by that of newly synthesized 18:0. The deuterium enrichment of body water was determined by isotopic exchange with [U-13C3] acetone as described previously.36
Total RNA was extracted from homogenized liver using an RNeasy kit (Qiagen, Germantown, MD, USA) following the manufacturer's instructions. Messenger RNA was then extracted from total RNA preparations using an Oligotex kit (Qiagen) following the manufacturer's instructions. The quality and integrity of the RNA were checked using the A260/280 ratio and electrophoresis on a formaldehyde/agarose gel, respectively. Equal amounts of RNA were reverse transcribed using Superscript II reverse transcriptase (Invitrogen, Carlsbad, CA, USA) as per the manufacturer's instructions. Primers for reverse transcriptase-PCR were designed using the primer design software Primer3, after which the sequence homology for related proteins was checked. Specifically, 18S ribosomal RNA primers were used as an endogenous control. Reverse transcriptase-PCR was performed on an ABI Prism 7700 Sequence Detection System (PE Applied Biosystems, Foster, CA, USA), and the data obtained were analyzed using the provided software. The reaction mixture consisted of 4 μl complementary DNA template, 10 μl Sybr Green PCR master mix (Roche Biochemicals, Indianapolis, IN, USA), 2 μl 0.25–1 μM forward primer and 2 μl 0.25–1 μM reverse primer in a 20 μl reaction volume. The PCR protocol consisted of a single 10 min denaturation cycle at 95 °C followed by 40 cycles of denaturation at 95 °C for 15 s and annealing/extension at 60 °C for 1 min. Standard curves for each gene and endogenous 18S ribosomal RNA control were obtained. The efficiency of PCR amplification was 100%, and the R2-value was between 0.995 and 0.999. All reverse transcriptase-PCR data were expressed as relative mRNA levels after normalization to 18S ribosomal RNA. Primer pair sequences are listed in Supplementary Table S3.
Data are presented as the means±s.e.m. unless otherwise indicated. Data were analyzed by one-way analysis of variance using Tukey's post hoc test to determine statistical significance for all pairwise multiple comparison procedures and Dunnett's test for multiple comparisons against the control group.
Effect of KAA on obese mice models
We first examined KAA fortification in C57B6 mice fed either the low-fat diet (LFD) or the lard-based HFD. Before the experiment, mice were fed either LFD or HFD for 2 months (pre-LFD or pre-HFD). At day 0, the average body weights of mice in the pre-LFD and -HFD groups were 31.6±0.3 and 37.1±0.5, respectively. Under pre-LFD conditions, the 4 weeks of high-KAA diets significantly reduced body weight gain (BWG) in both LFD and HFD (Figure 1a right panel and Figure 1b). In pre-HFD conditions, however, the high-KAA diet reduced BWG only in LFD, but no clear reduction was seen in HFD. Table 1 summarizes weights of the liver, kidney, gastrocnemius and soleus muscle as well as the different part of adipose tissues at the end of experiment. No significant changes in these tissue weights were observed, except for adipose. During the experimental period, KAA fortification of the HFD had no effect on food intake, but reduced the amount of food intake on the LFD. KAA fortification of the HFD increased oxygen consumption without changes in the respiratory quotient compared with the control HFD (Figures 1d and e).
Under pre-LFD conditions, the high-KAA diets significantly reduced postprandial insulin and fat accumulation for both the LFD and the HFD. The pre-HFD, high-KAA diets, however, reduced those two parameters only under the LFD condition, but had no effect under HFD conditions (Figure 2a). Unlike plasma insulin and fat accumulation, the high-KAA diets reduced hepatic fat contents in all conditions, with more significant reductions under HFD conditions than under LFD conditions (Figure 2a, bottom). To further understand the associations between postprandial insulin and both hepatic and adipose fat accumulations, we examined dietary KAA fortification in hyperinsulinemic ob/ob mice. The ob/ob mice were fed an HFD or LFD for 2 weeks with or without dietary KAA fortification. In ob/ob mice, the high-KAA diet reduced postprandial insulin only in the LFD (Figure 2b). The KAA diets significantly reduced hepatic fat conditions under both the LFD and the HFD. Similarly, in C57B6 mice under HFD conditions, the reduction due to the high-KAA diet was more significant in improving hepatic steatosis than under the LFD (Figures 2b and c). The dietary KAA fortification did not affect body fat content in ob/ob mice after at least 2 weeks of feeding (Figure 2b).
Effect of KAA on varying dietary lipid-induced metabolic phenotypes
These metabolic changes under dietary KAA fortification in both C57B6 and ob/ob mice suggest that KAA fortification predominately affects hepatic fat rather than adipose fat contents, and it is more effective under high-fat conditions. To address the relationship between dietary KAA and fatty types, we next compared three different KAA-supplemented HFDs, namely, PO-, FO- or SO-based diets. The control LFD was prepared by blending the three oils.
Dietary lipids of these three different oils were analyzed by GC-MS to confirm their fatty acid compositions (Figure 3a). More than half of the fatty acids in the PO were SFA, of which nearly 50% were palmitate (16:0) and 5% were stearate (18:0). The FO was mostly MUFA, of which over 80% was oleate. The SO consisted primarily of PUFA, of which 52% was linoleate (18:2) and 6% was linolenate (18:3).
Table 2 illustrates the postprandial variables at the end of the 8-week experimental period. The high-KAA diet significantly reduced postprandial plasma cholesterol in the high-PO and high-FO conditions, whereas no clear reduction was observed in mice consuming the high-SO diet. Although HFD feeding caused only slight increases in blood glucose and TG in comparison to the LFD group, the high-KAA diet almost normalized these values in mice consuming the HFDs (Table 2). Under these conditions, no significant changes in food intake were observed between control, high-fat and KAA fortified groups (Figure 3b). BWG due to high-PO or high-SO feeding was significantly repressed by KAA fortification, whereas no significant increase in BWG on high-FO diets or repression by KAA feeding was observed (Figure 3c). At the end of the 8-week experimental period, the epididymal fat weight decreased by 34% in the KAA group as compared with both the control PO and the SO groups (Figure 4c).
Effect of KAA on hepatic lipid contents with varying dietary lipids
As compared with the level in the control LFD group, hepatic TG content was increased by 75 and 29% under the high-PO and high-FO diets, respectively, whereas no significant increase was observed under the high-SO diet (Figure 4c). Similar trends were observed regarding hepatic cholesterol content, which increased by 26 and 43% under the high-PO and -FO diets. However, KAA fortification of both high-PO and -FO diets repressed increases in both hepatic TG and cholesterol. There were no clear changes in hepatic TG and cholesterol contents in high-SO groups compared with the control LFD group (Figure 4c).
De novo lipogenesis and lipid partitioning
To understand the mechanism of TG regulation under the high-KAA condition, metabolic flux analysis was used to quantify changes in DNL and non-DNL lipid partitioning to tissues. Figure 5 summarizes the different fatty acid sources contributing to hepatic and adipose TG in C57B6 mice fed various diets for 8 weeks.
In fat tissue, the contribution of DNL to palmitate and oleate contents was generally smaller and lower in all HFD groups as compared with the control LFD group (Figure 5, right panels). In contrast, a large contribution of DNL to palmitate and oleate synthesis in the liver was observed under both high-PO and high-FO diets and in the control LFD group; this effect was significantly reduced in mice consuming the high-SO diet (Figure 5, left and right panels). The different dietary oils also showed different patterns of non-DNL partitioning and accumulation in both tissues, presumably from different dietary fatty acids. Particularly in the liver, high levels of PO, FO and SO increased non-DNL palmitate, oleate and linoleate, respectively.
KAA supplementation in high-PO and high-FO diets significantly reduced the DNL of palmitate and oleate and the non-DNL partitioning of these two fatty acids into the liver (Figure 5, left panels). KAA supplementation under the high-SO condition, however, failed to reduce the hepatic DNL and TG. Interestingly, KAA significantly reduced SO-induced accumulation of linoleate, but increased the non-DNL oleate in both tissues (Figure 5). In contrast, KAA reduced FO-induced non-DNL oleate, but increased linoleate (Figure 5).
Changes in hepatic lipogenic gene expression by dietary fat and amino acids
Expression of hepatic genes involved in lipogenesis was measured in response to varying HFD feeding with or without KAA supplementation (Figure 6). The high-KAA diet repressed the high-PO induced increase in the sterol regulatory element-binding protein-1c (SREBP-1c), but failed to repress expression under high-FO and high-SO diets. Expression of adenosine triphosphate citrate lyase (ACL), acetyl-CoA carboxylase (ACC), stearoyl-CoA reductase (SCD-1) and Elovl-6 was reduced under all three HFDs as compared with the control LFD group, whereas KAA supplementation additively repressed the expression of these enzymes, particularly in both high-PO and high-FO diets (Figure 6). The high-SO diet dramatically decreased ACL, ACC and SCD-1 expression by 70–90% as compared with the LFD group; no additional effect due to KAA was observed. Fatty acid synthase (FAS) expression was reduced in all HFDs, and no clear effect of KAA supplementation was observed (Figure 6). Regarding glucolytic genes, only the high-PO diet increased the expression of glucokinase (GK) genes, and KAA repressed such expression. In addition, no clear changes due to KAA were observed in liver pyruvate kinase.
Correlation of lipogenic fluxes and gene expression
To understand the regulatory differences of lipogenic genes induced by dietary lipid and amino acids, we performed correlation analyses of lipogenic fluxes and gene expression patterns. In this study, we estimated elongase and desaturase fluxes in addition to palmitate synthesis (DNL of palmitate), as shown in Figure 5, and then we compared these fluxes to the expression of the lipogenic genes ACL, ACC, FAS, Elovl-6 and SCD-1. Figure 7 shows the correlation between palmitate synthetic flux and related expression patterns of ACL, ACC and FAS. The flux of palmitate synthesis shows a relatively high correlation with ACL and ACC (r=0.53 and 0.38, respectively), whereas no clear correlation with FAS was seen. Correlations between elongase flux and Evovl-6 expression and between desaturase flux and SCD-1 expression were also assessed; the desaturase reaction, but not the elongase reaction, exhibited a correlation between flux and expression patterns (Figure 7).
This study found that dietary lipids and amino acids reciprocally affect fat accumulation in mice through the regulation of DNL and tissue lipid distribution. Increased intake of nutritional elements such as carbohydrates and fat has been reported to lead to obesity and insulin resistance.3, 4 Several studies have suggested that dietary fatty acid composition affects the development of insulin resistance, hepatic steatosis and obesity.10 Different types of fatty acids display different metabolic phenotypes, including oxidation and deposition rate differences that lead to body fat changes.37 The chemical structure of dietary fatty acids and their chain length, degree of unsaturation, the position of double bonds and their configuration seem to affect their metabolic fate. For example, one comparison of dietary MUFA intake with SFA revealed a decrease in fat deposition under a diet rich in MUFA.38 For unsaturated long-chain fatty acids, PUFA from fish oil has been reported to decrease fat mass in rodents.39
To address these issues, we examined the effects of three different diets high in PO, FO and SO on lipid metabolism in C57B6 mice, where PO, FO and SO predominantly contained SFA, MUFA and PUFA, respectively. Our data show clear differences in fat accumulation among these dietary groups; both PO and SO (but not FO) increased BWG in mice. In addition, PO induced fat accumulation in both liver and adipose tissue, whereas FO and SO only induce it in liver and adipose tissue, respectively. These differences in fat accumulation in tissues can also be explained according to the different types of dietary fat and their behaviors in lipid metabolism. For instance, in vivo and in vitro studies have shown that PUFA, but not MUFA nor SFA, seems to suppress the expression of lipogenic genes primarily through decreased expression of SREBP-1c.40 Our data show that all three oils increase SREBP-1c expression in mice, but strongly repress downstream genes such as SCD-1 and Elovl-6. The differences in the expression of SREBP-1c and other lipogenic genes based on different HFDs were not clear in this study. Both the proportions of dietary fatty acid types and the duration of treatment may further complicate the effects on lipid metabolism.
Recent studies have shown that dietary protein could affect fat accumulation by satiating and metabolic effects.41 In addition, amino acid, fat and glucose metabolisms are highly coordinated through multiple organ systems, including the liver.25, 42, 43 However, the mechanism by which dietary amino acids regulate lipid metabolism is still unclear. We previously reported that the manipulation of the essential amino acid/non-essential amino acid ratio by supplementation with both the KAA lysine and threonine and the branched-chain amino acids prevented hepatic steatosis through repression of DNL in mice.30 To extend this finding, we examined the effect of KAA supplementation on the murine lipid synthetic pathway as well as on the fat deposition that occurs when mice are fed different HFDs. In this study, we replicated our previous findings on the reduction of hepatic lipid by dietary KAA in C57B6 mice, as we investigated KAA fortification under LFD and HFD in mice. Our data clearly duplicated a reduction in hepatic and body fat due to KAA, with increased oxygen consumption under HFD conditions. However, we found that KAA supplementation had relatively less of an effect under LFD conditions, although it introduced a slight anorexic effect under LFD. Therefore, we hypothesized that the reduction of fat accumulation by dietary KAA could be partly dependent on dietary fat content or fatty types. Our data interestingly showed that KAA supplementation exhibited a clear dependency on dietary fatty acid types in terms of the repression of fat deposition; KAA only decreased hepatic TG and cholesterol content in high-PO and high-FO diets. This difference was also observed for lipogenic gene expression. KAA supplementation of the high-PO diet decreased the expression of SREBP-1c and SCD-1, and KAA supplementation of the high-FO diet decreased the expression of SCD-1 and Elovl-6. However, KAA supplementation of the high-SO diet did not alter the expression of lipogenic genes, suggesting that these amino acids utilize some of the same factors as PUFA to regulate lipid metabolism. As compared with the high-FO diet, the high-PO diet dramatically increased hepatic GK expression, and this increase was normalized by KAA supplementation. Differences in glycolytic regulation by fatty acids have been reported in vitro, where palmitate, but not oleate, directly represses GK activity or flux in liver cells.29, 44 In addition, SERBP-1c has been reported to modulate insulin-dependent GK regulation, indicating the parallel regulation of glycolysis and lipogenesis.45 The current data do not address the mechanism by which GK is regulated by dietary lipid or amino acids; thus, further study of the combined effect of fatty acids and amino acids on the regulation of hepatic glycolysis is needed.
DNL is normally assessed by profiling the expression of lipogenic genes. However, such analyses do not cover all possible regulatory mechanisms of the pathway because regulation could also occur independently of gene expression. For example, regulation can also occur through changes in substrate availability, in the phosphorylation state of the enzymes or in allosteric regulation.46 Therefore, metabolic flux analysis should be used to describe the activity or inactivity of the DNL pathway. In this study, we examined both metabolic flux analysis and gene expression. Although lipogenic gene expression was altered by dietary conditions, correlation analysis extracted a limited relationship between gene expression and actual fluxes. For instance, a positive relationship was observed between desaturase flux and SCD-1 expression. In contrast, no clear correlation was observed between elongase flux and Elovl-6 expression, although significant changes in gene expression were observed. Furthermore, the DNL flux of palmitate showed a clear correlation with ACL and ACC expression, but not with FAS expression. Kotronen et al.47 reported that SCD-1, but not elongase activity, was positively correlated with hepatic fat in non-alcoholic fatty liver diseased patients. The current data strongly indicate that DNL can be regulated by changes in gene expression as well as by changes in flux due to substrate availability due to dietary components, where amino acids may alter the upper pathway of lipogenesis and the desaturase fluxes.
Another important finding in this study is that tissue lipid distribution seems to be modulated by KAA supplementation, particularly in high-FO and high-SO diets. Our data show that KAA significantly reduced SO-induced hepatic and adipose accumulation of linoleate (18:2), although increased oleate (18:1) was observed in both tissues. However, KAA reduced FO-induced oleate accumulation in both tissues, but increased linoleate accumulation in adipose tissue. The mechanism underlying this exchange of tissue fatty acids with amino acids is unclear. However, fatty acid-binding proteins and acyl-CoA binding protein might be involved in these phenomena because these proteins determine whether lipid metabolites are used as an energy source or as signaling molecules within cells. They also regulate the circulation of lipid metabolites, which affects the tissue distribution of lipids.48 The KAA used in this study are known to generate short or branched chain acyl-CoAs that might disturb interactions with long-chain fatty acids. In addition, several studies have examined the decreased expression of intestinal fatty acid-binding protein and fatty acid transport protein-4 induced by branched-chain amino acids in human intestinal cells.49 Of course, there may be additional factors that sense the proportion of fatty acids and amino acids in diets that regulate hepatic lipid metabolism. Thus, further metabolic profiling of amino-acid metabolism may be a possible approach to relate such metabolites to the metabolic fate of lipids and to the regulation of de novo lipid synthesis.
We studied KAA fortification in C57B6 mice after 2 months of LFD or HFD feeding. We found that KAA fortification mitigated the reduction in body fat in the pre-HFD-treated mice. Because we previously found that dietary KAA prevented high-fat-induced peripheral insulin resistance through the reduction of lipotoxic lipid accumulations,30 the irreversible development of peripheral insulin resistance and the subsequent impairment in substrate oxidation by long-term HFD feeding may explain it. In contrast to adipose fat, KAA fortification was effective in the reduction of hepatic fat in pre-HFD mice as well as in hyperinsulinemic ob/ob mice. Thus, the regulation of hepatic lipid accumulation by KAA was independent of diet-induced insulin resistance.
In rodents, the anorexic effects of KAA loading must be considered. The accompanied decrease in caloric intake distorts metabolism as a whole, making the interpretation of experimental results difficult. Leucine, methionine and histidine have been characterized as having a strong, negative influence on food intake in rodents.50 Among these, leucine was reported to stimulate mammalian target of rapamycin signaling directly in the hypothalamus, leading to decreased food intake.51, 52 In addition, amino-acid imbalance caused by supplementing either a single amino acid or a few specific amino acids negatively impacts the so-called ‘metabolic value’ of the diet in question. Taken together, these factors have largely confounded previous attempts to assess the direct or upstream metabolic effects of KAA. In this study, we did not observe a reduction in food intake associated with feeding a mixture of selected KAA to mice under HFD conditions, suggesting that the utilization of multiple KAA, together with dietary fat, could alleviate the potential for anorexic effects. This mixture was composed of free BCAA plus lysine and threonine, which quantitatively are the major KAA in most animal proteins. Although further optimization of our formulation is required to elucidate the contribution of each individual amino acid, the KAA diet developed in this study exhibits a marked capacity to modulate high-fat-induced metabolic alterations and to prevent subsequent pathogenesis.
In conclusion, KAA may regulate DNL through a regulatory mechanism similar to that used for PUFA, but regulation by KAA could also occur through pathways independent of regulation by fatty acids. In addition, the modulation of lipid partitioning could be another factor explaining the lipid-reducing effect of KAA.
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Supplementary Information accompanies the paper on the Nutrition and Diabetes website (http://www.nature.com/nutd)