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S. Polakof, F. Médale, L. Larroquet, C. Vachot, G. Corraze and S. Panserathigh-carbohydrate diet
Regulation of de novo hepatic lipogenesis by insulin infusion in rainbow trout fed a
published online May 13, 2011J ANIM SCI
http://jas.fass.org/content/early/2011/05/13/jas.2010-3733the World Wide Web at:
The online version of this article, along with updated information and services, is located on
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Regulation of de novo hepatic lipogenesis by insulin infusion in rainbow trout
fed a high-carbohydrate diet1
S. Polakof*#1, F. Médale*, L. Larroquet*, C. Vachot*, G. Corraze,* and S. Panserat*
* INRA, UR1067 Nutrition Metabolism Aquaculture, F-64310 Saint-Pée-sur-Nivelle, France
#Laboratorio de Fisioloxía Animal, Departamento de Bioloxía Funcional e Ciencias da Saúde,
Facultade de Bioloxía, Universidade de Vigo, E-36310 Vigo, Spain.
1Acknowledgements
This study was supported by research grants from Agence Nationale de la Recherche
(ANR-08-JCJC-0025-01) and INRA Animal Physiology – Livestock Systems (PHASE)
Department. S. Polakof was the recipient of a postdoctoral fellowship from the Xunta de Galicia
(Program Ángeles Alvariño). We thank the technical staff (Y. Hontang, F. Sandres, and F.
Terrier) of the INRA experimental fish farm of Donzacq for supplying the experimental animals.
2Corresponding author:
Dr. Sergio Polakof
INRA, UR1067 Nutrition Metabolism Aquaculture, Pôle d’hydrobiologie, CD918, F-64310 St-
Pée-sur-Nivelle, France
Tel: (33) 5 59 51 59 60; Fax: (33) 5 59 54 51 52; e-mail: [email protected]
Present adress: INRA, UMR 1019, UNH, CRNH Auvergne, Clermont-Ferrand, France;
Clermont Université, Université d’Auvergne, Unité de Nutrition Humaine, Clermont-Ferrand,
France
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Abstract
Carbohydrate energy intake in excess of total energy expenditure is converted to fat. In
fish, the liver is considered to be the main lipogenic tissue. Its regulation by insulin is not fully
understood and some of the available in vivo findings are contradictory. In this study, bovine
insulin was infused for 5 d into rainbow trout fed a high-carbohydrate diet and parameters of de
novo hepatic lipogenesis were measured. We found that hepatic lipogenesis in trout is stimulated
by insulin, reflected in enhanced mRNA and protein levels and enzyme activity of ATP-citrate
lyase, acetyl-CoA carboxylase, and fatty acid synthase. These results were further supported by
parallel changes in enzymes acting as NADPH donors, especially those participating in the
pentose phosphate pathway. This is the first time that the main enzymes involved in de novo
hepatic lipogenesis have been studied at molecular, protein, and activity levels in fish. We
hypothesize that some of the delayed changes found in the different levels of regulation were
probably related to the insulin resistance achieved by the trout liver after 5 d of insulin infusion.
We assessed enzyme activity and mRNA levels of lipid oxidation-related enzymes in the livers
of insulin-infused fish in which paradoxically increased β-oxidation potential was found. The
insulin-stimulated de novo hepatic lipogenesis in carbohydrate-fed trout reinforces the
hypothesis that this pathway may act as an important sink for an excess of glucose, which could
ultimately contribute to improved glucose homeostasis in this carnivorous and ‘glucose-
intolerant’ species when fed high-carbohydrate diets.
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Key Words: dietary carbohydrate, fish, insulin, lipogenesis, liver
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INTRODUCTION
As in rainbow trout (Oncorhynchus mykiss), de novo hepatic lipogenesis (DNL) in
salmonids, is regulated by several factors, including nutritional status (Lin et al., 1977a), energy
content in the diet (Kolditz et al., 2008), genetic background (Skiba-Cassy et al., 2009), anti-
diabetic drugs (Panserat et al., 2009; Polakof et al., 2011b), macronutrients (Álvarez et al., 2000),
migration processes (Sheridan et al., 1985), and hormones (Cowley and Sheridan, 1993; Higgs et
al., 2009).
Insulin stimulates synthesis of fatty acids and triacylglycerols and enhances
triacylglycerol storage in the liver through long-term effects on the expression of lipogenic
genes, and this is often accompanied by inhibition of fatty acid oxidation in mammals (Kersten,
2001). The picture is unclear in fish, where the insulin effects reported are contradictory and the
mechanisms of insulin regulation have not been fully elucidated (Machado et al., 1988; Pérez-
Sánchez, 1988; Plagnes-Juan et al., 2008; Polakof et al., 2010b; Polakof et al., 2009). Recent
findings suggest a major role of DNL in glucose homeostasis, including a better glycemic profile
in trout treated with metformin (Panserat et al., 2009; Polakof et al., 2011b) and in genetically
selected lines (Skiba-Cassy et al., 2009). To obtain greater understanding of the effects of insulin
on hepatic DNL under physiological conditions, we infused rainbow trout with insulin for 5 d.
Due to the anabolic action of this hormone (Navarro et al., 2006), we hypothesized that insulin at
physiological doses would stimulate DNL in order to store the excess circulating glucose. We
assessed the activity, protein and mRNA levels of key enzymes involved in lipogenesis as well
as the main enzymes acting as NADPH donors. Tissue insulin sensitivity was estimated on the
basis of the phosphorylation status of Akt/PKB, a critical node in the insulin signaling pathway
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in both fish (Seiliez et al., 2008) and mammals (Taniguchi et al., 2006). Insulin-regulated lipid
metabolism was examined through measurement of representative lipid oxidation enzymes.
MATERIALS AND METHODS
The experiments were conducted following the Guidelines of the National Legislation on
Animal Care of the French Ministry of Research (Decret Nº 2001-464, May 29, 2001) and were
approved by the Ethics Committee of INRA (according to INRA 2002-36, April 14, 2002).
Fish
Rainbow trout (Oncorhynchus mykiss Walbaum) were obtained from the INRA
experimental fish farm facilities of Donzacq (Landes, France). Fish were maintained in tanks
kept in open recirculated circuits with 17°C well-aerated water and controlled photoperiod
(LD12:12), and fed a standard trout commercial diet during the acclimation period (T-3P classic,
Trouw, France; crude protein = 49.8% dry matter, crude fat = 13.8% dry matter; gross energy =
22 kJ/g dry matter). Mean fish weight was 200 ± 10 g.
Experimental Protocols
For sustained hormone infusions, fish were feed-deprived for 48 h and then implanted
with 1003D Alzet mini-osmotic pumps (ALZED Osmotic Pumps, Cupertino, CA) containing
either saline (control, n = 12) or bovine insulin (Sigma Chemical Co., St. Louis, MO) solution (n
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= 12) at 2 doses. Fish were anesthetized, BW measured, and pumps inserted into the peritoneal
cavity through a 1.0-cm incision made in the ventral midline at ca. 2.0 cm rostral of the pelvic
fins. The incision was closed with 1 stitch and an antibiotic gel was applied topically to the
incision area. Pumps were implanted in the morning and fish were allowed to recover for 24 h.
Fish were then hand-fed once daily at 2% BW with a diet containing a high level of carbohydrate
(30% dextrin, 57% fish meal, and 10% fish oil) for 5 d and sampled 6 h after their last meal.
Pump flow rate was established to be 0.39 L·h-1, which at 17ºC should provide sustained
release of 0.35 or 0.7 insulin IU·kg-1·d-1. The doses and heterologous insulin used in the present
study were selected on the basis of previous studies (Plisetskaya et al., 1993; Polakof et al.,
2009).
Tissue and Blood Sampling
Trout were sacrificed by a sharp blow on the head. Blood was removed from the caudal
vessel and centrifuged (3,000 × g, 5 min, 4ºC). Plasma was frozen at -20ºC pending analyses.
The gut contents of each fish were systematically checked to confirm that the fish being sampled
had consumed the diet. Livers were collected and frozen in liquid nitrogen and stored at -80°C
pending analyses, except for 1 piece of each liver that was immediately homogenized to assess
carnitine palmitoyltransferase (CPT1) activity (see below).
Molecular and Biochemical Analyses
Plasma glucose (Biomérieux, Marcy l'Etoile, France), triglycerides (Biomérieux), and
NEFA (NEFA C from Wako Chemicals GmbH, Neuss, Germany) levels were determined using
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commercial kits adapted to a microplate format (Polakof et al., 2010a, 2011b). Bovine insulin
levels were measured in trout plasma using a bovine-specific commercial ELISA kit (Mercodia,
Sweden) according to Polakof et al. (2009).
Tissue mRNA levels encoding proteins involved in lipid and energy metabolism were
determined by realtime quantitative RT-PCR (qPCR; Polakof et al., 2010a). Total RNA was
extracted from livers using TRIzol reagent (Invitrogen, Carlsbad, CA) according to the
manufacturer's recommendations. One microgram of the resulting total RNA was reverse
transcribed into cDNA using the SuperScript III RNaseH- Reverse Transcriptase kit (Invitrogen)
and random primers (Promega, Charbonnières, France) according to the manufacturer’s
instructions. Realtime RT-PCR was carried out with an iCycler iQ realtime PCR detection
system (BIO-RAD, Hercules, CA) using iQ SYBR Green Supermix. The transcripts assessed
were acetyl-CoA carboxylase (ACC), fatty acid synthase (FAS), ATP-citrate lyase (ACLY),
glucose 6-phosphate dehydrogenase (G6PDH), 6-phosphogluconate dehydrogenase (6PGDH),
malic enzyme (ME), and isocitrate dehydrogenase (ICDH). Primers were designed to overlap an
intron where possible (Primer3 v. 0.4.0 software; http://frodo.wi.mit.edu/primer3/#disclaimer;
Rozen and Skaletsky, 2000) using known sequences found in trout nucleotide databases
(Genbank and INRA-Sigenae) as previously described (Ducasse-Cabanot et al., 2007; Polakof et
al., 2010a, 2011a). The transcript level of elongation factor 1α (EF1) was stably expressed in
this study. Relative quantification of the target gene transcript with the EF1 reference gene
transcript was made following the Pfaffl method (Pfaffl, 2001). The relative expression ratio (R)
of a target gene was calculated on the basis of realtime PCR efficiency (E) and the CT deviation
(ΔCT) of the unknown sample compared to a control sample and expressed in comparison to the
EF1 reference gene: R = [(Etarget gene)ΔCt target gene (mean control-mean sample)/(Eef1α)
ΔCt ef1α(mean control-mean
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sample)]. Efficiency (E) of PCR was measured by the slope of a standard curve using serial
dilutions of cDNA.
Western blotting (20 µg protein extracted from the liver) was undertaken using anti-
phospho-Akt Ser473 (Cell Signaling Technology, Ozyme, St Quentin-en-Yvelines, France), anti-
FAS (Santa Cruz Biotechnology, Santa Cruz, CA), anti-ACLY (Cell Signaling Technology),
anti-phospho-ACC Ser79 (Upstate, Euromedex, Munolsheim, France) and anti-β-tubulin (Cell
Signaling Technology). All antibodies were raised against human protein, except for Akt/PKB,
which was raised against mouse protein. Briefly, frozen livers (300 mg) were homogenized on
ice with an Ultraturrax homogenizer in a buffer containing 150 mM NaCl, 10 mM Tris , 1 mM
EGTA, 1 mM EDTA (pH 7.4), 100 mM sodium fluoride, 4 mM sodium pyrophosphate, 2 mM
sodium orthovanadate, 1% Triton X-100, 0.5% NP-40-IGEPAL, and
cOmplete,ULTRA,Mini,EDTA-free,EASYpack Protease Inhibitor Cocktail (Roche, Basel,
Switzerland; 1 tablet / 5mL) (4-(2-Aminoethyl)-benzenesulfonyl fluoridehydrochloride,
polyethylene glycol, polyvinylpyrrolidone, N-alpha-p-Tosyl-L-lysine chloromethyl ketone
hydrochloride, benzethonium chloride, D-Mannitol, phenylmethylsulfonyl fluoride).
Homogenates were centrifuged for 15 min at 12,000 × g, 4ºC and the resulting supernatants
stored at -80ºC. Protein concentrations were determined using the Bio-Rad protein assay kit
(BIO-RAD). Protein lysates (20 μg) were subjected to SDS-PAGE and Western blotting using
the appropriate antibody. After washing, membranes were incubated with an IRDye infrared
secondary antibody (LI-COR Biotechnology, Lincoln, NE). Bands were visualized by infrared
fluorescence using the Odyssey imaging system (LI-COR Biotechnology) and quantified by
Odyssey infrared imaging system software (version 1.2). The signal of each protein was
normalized to the β-tubulin signal. Validation of Akt/PKB and FAS mammalian antibodies was
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previously demonstrated in the trout (Seiliez et al., 2008; Polakof et al., 2010a). The trout ACLY
(GAY7CUQ01A40MK.s.om.10, CA349411.s.om.10) AA sequence is 90% homologous to
human ACLY (NP_001087.2), while the trout FAS (Sigenae database, GAY7CUQ02F6SW9)
AA sequence is 88% homologous to human FAS (NP_004095.4). As in the rat ACC
(NP_071529.1), a serine was also found in the trout ACC protein (Sigenae database,
FYV3OTN01B4R4N.s.om.10).
Livers used to assess enzyme activities were homogenized with ice-cold buffer (10
wt/vols; 20 mM Tris, pH 7.4, 250 mM sucrose, 2 mM EDTA, 10 mM β-mercaptoethanol, 100
mM NaF, 0.5 mM EDTA). The homogenate was centrifuged for 20 min at 17,000 × g, 4ºC and
the supernatant used immediately for enzyme assays. Hydroxyacyl-CoA dehydrogenase (HOAD)
and ACC were assessed as in Kolditz et al. (2008), while G6PDH and FAS were assessed
following the method described by Figueiredo-Silva et al. (2010) adapted to trout tissues. Levels
of enzyme activity of ME and 6PGDH were assessed as in Mommsen et al. (2003) adapting the
substrate liver concentration: 0.5 mM phosphogluconic acid for 6PGDH and 0.08 mM malic acid
for ME. Enzyme activity of ACLY was determined as in Álvarez et al. (2000). Total CPT1
activity was assessed on fresh tissue as in Gutieres et al (2003). Enzyme activity levels are
expressed in terms of mg protein. Protein concentrations were determined using a Bradford
protein assay kit (Bio-Rad, Germany) with BSA as standard (Bradford, 1976).
.
Statistical Analysis
Results are expressed as means ± SEM. (n = 6). Data were analyzed by one-way
ANOVA. When necessary, data were log-transformed to fulfill the conditions of the analysis of
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variance. Post-hoc comparisons were made using a Student-Newman-Keuls test, and differences
were considered statistically significant at P < 0.05.
RESULTS
Plasma glucose levels in the group receiving the lower insulin dose were less (P = 0.029)
than in the other 2 groups (control and higher insulin dose), while in the higher dose group (P >
0.10) glycemia was similar to the saline-infused group. Plasma triglyceride levels were
unaffected (P > 0.10) by insulin infusion when compared with the saline-infused group. In
contrast, free fatty acid levels in plasma were reduced after insulin infusion (P = 0.011 and 0.046
respectively). Bovine insulin levels were 2-fold higher in the animals infused with the 0.7 IU·kg-
1·d-1 insulin dose than in those receiving 0.35 IU·kg-1·d-1 insulin (P = 0.024).
The phosphorylation status of liver Akt/PKB Ser473 was unchanged (P > 0.10) by insulin
infusion (Figure 1).
Liver ACLY, ACC, and FAS enzyme activities, protein, and mRNA transcript levels are
shown in Figure 2. No changes were observed (P > 0.10) in ACLY activity irrespective of the
insulin dose. Low dose insulin increased (P = 0.016) ACLY mRNA 2-fold compared to controls.
High-dose insulin increased (P = 0.033) ACLY protein compared to saline controls. Both protein
(P = 0.039) and activity levels (P = 0.013) of ACC were upregulated in fish receiving 0.7 IU·kg-
1·d-1 insulin. No changes (P > 0.10) in ACC mRNA levels were noted in the control group. The
levels of FAS mRNA levels were upregulated (P = 0.048) by insulin, only at the 0.35 IU·kg-1·d-1
dose. The protein and activity levels of FAS were unaffected (P > 0.10) by the low dose of
insulin treatment, and increased (P = 0.034) by the higher-insulin dose.
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Changes in enzyme activity and mRNA levels of proteins acting as NADPH donors in the
liver are shown in Figure 3. Levels of enzyme activity of 6PGDH, G6PDH, and ME were
increased (6PGDH, P = 0.009; G6PDH, P = 0.001; ME, P = 0.05) by insulin. Transcript levels
for 6PGDH were upregulated (Ins0.35, P < 0.001; Ins0.7, P = 0.009) in a dose-dependent
manner.
Changes in activity levels of enzymes involved in lipid oxidation pathways in the liver
are shown in Table 2. The level of activity of HOAD was increased in trout infused with the
hormone independently of the insulin dose (P = 0.048 for 0.35; P = 0.021 for 0.7), whereas no
changes in mRNA levels were noted (P > 0.10). No changes in levels of CPT1 activity were
noted in any of the insulin-infused groups (P > 0.10), although mRNA levels increased with the
higher-insulin dose for CPT1A (P = 0.025) and increased with both insulin doses for CPT1B (P =
0.017 for 0.35; P = 0.025 for 0.7).
DISCUSSION
Insulin-stimulated DNL Potential in Rainbow Trout Liver
Although the role of adipose tissue in DNL remains to be elucidated in fish (Polakof et
al., 2011a), the liver has been traditionally considered to be the main lipogenic organ in many
fish species, including salmonids (Henderson and Sargent, 1985). In the study presented here, we
analyzed important enzymes involved in DNL, including ACLY, ACC, and FAS. This is the first
global assessment of insulin regulated-DNL in the trout liver to date.
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Despite the lack of changes in the relative phosphorylation status of Akt/PKB in our
study, significant changes were noted in DNL-related enzymes. The fact that Akt/PKB was
unaffected by the insulin infusion 6 h after feeding does not mean that the effects observed here
were Akt/PKB-independent, since earlier phosphorylation of this protein has been reported in the
postprandial state (Seiliez et al., 2008; Skiba-Cassy et al., 2009). It should be borne in mind that,
despite the presence of insulin receptors, the liver is not a highly insulin-sensitive tissue
(Gutiérrez et al., 2006; Navarro et al., 2006). We cannot rule out that some degree of insulin
resistance may be induced by insulin infusion in this species (Polakof et al., 2010c) or that there
is insufficient stimulation of the trout Akt/PKB systyem by heterologous insulin. This may
explain the lack of hyperglycemia with the higher insulin dose and some of the differences
between the molecular and biochemical regulation of the enzymes studied.
The primary enzyme responsible for the synthesis of cytosolic acetyl-CoA is ACLY.
Although its activity and gene expression have already been described for fish liver, this is the
first time that insulin regulation of the enzyme has been assessed in vivo. We found enhanced
ACLY mRNA levels in fish receiving the lower-insulin dose, while protein levels were
upregulated with the higher-insulin dose. These differences between mRNA and protein levels
may be due to delayed protein synthesis after increased transcript production, although we
cannot eliminate the possibility of an insulin-resistance effect with the higher-hormone dose.
Further support for this phenomenon could be found in the different regulation of ACLY mRNA
levels (unchanged; Lansard et al., 2010) and activity (increased; Álvarez et al., 2000) in trout
hepatocytes stimulated with both insulin and glucose. The lack of changes in activity in the
present study may have been due to increased citrate levels from the tricarboxylic acid cycle or
changes in the phosphorylation status of the protein (Potapova et al., 2000). Our results also
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agree with the regulation described for this enzyme in mammals, where ACLY is stimulated in
the presence of insulin and glucose (Fukuda and Iritani, 1999).
The formation of malonyl-CoA, an essential substrate for FAS and fatty acid chain
elongation in DNL, is catalyzed by ACC. We observed complex regulation of ACC in the livers
of rainbow trout, based upon gene expression analysis, protein phosphorylation profiles, and
enzyme activity measurements. The findings confirm the presence of a functional ACC in the
trout liver, supporting previous studies in which ACC activity was increased in trout fed high
carbohydrate (Rollin et al., 2003) or low energy (Kolditz et al., 2008) diets. As stated above,
insulin stimulates the hepatic lipogenic pathway in mammals. While no changes in gene
expression were noted, both the phosphorylation on the Ser79 and activity were clearly
upregulated in those trout receiving the higher-insulin dose. It is possible that a transient increase
in ACC transcription occurred over the 5-d infusion period that could account for the elevated
enzyme activity. Although ACC activity in trout is increased in glucose and insulin-stimulated
hepatocytes (Álvarez et al., 2000), no information is available regarding the phosphoregulation
of ACC in fish. In mammals, AMP-kinase phosphorylation of ACC on Ser79 leads to inhibition
of enzyme activity, and insulin-stimulated dephosphorylation of the serine causes an increase in
liver ACC activity (Witters and Kemp, 1992). The fact that in the present study insulin seems to
increase ACC activity despite the enhanced phosphorylation status on Ser79 suggests that the
regulation of this enzyme in trout is complex and probably different from the mammalian model.
In mammals and birds, FAS gene expression, protein, and activity levels are upregulated
in the presence of insulin (Griffin and Sul, 2004; Radenne et al., 2008). We observed that FAS
activity is also upregulated by insulin, suggesting that the regulation by both insulin and glucose
is similar in the trout to that reported in other vertebrates. These results agree with previous
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findings obtained in fed trout subjected to similar treatments (Polakof et al., 2011b). The amount
of FAS mRNA (Lansard et al., 2010) and activity (Álvarez et al., 2000) are upregulated in
glucose- and insulin-stimulated trout hepatocytes.
Insulin Regulates NAPDH Donors in Rainbow Trout Liver
The DNL in the cytoplasm of vertebrate cells requires a carbon source (acetyl-CoA) and
reducing equivalents (NADPH) produced by 1 or more of 4 cytoplasmic dehydrogenases
(G6PDH, 6PGDH, ICDH, and ME). All these enzymes have been characterized in the liver of
different fish species, including salmonids (Baldwin and Reed, 1976; Walton and Cowey, 1982).
The mRNA and levels of enzyme activity of the 4 NADPH donors in the trout liver were
measured. Activity levels were in the same range as reported by others (Lin et al., 1977b; Kolditz
et al., 2008), with ME exhibiting the lowest level of activity. Insulin enhanced the activity of all
the enzymes acting as NADPH donors, except for ICDH, which remained unaffected. The fact
that these enzymes are mainly affected at similar activity levels as the lipogenic ACLY, ACC,
and FAS suggests a minor molecular regulation by insulin for these enzymes and confirms the
importance of the NADPH donors for DNL in fish liver (Lin et al., 1977b; Aster and Moon,
1981). The higher levels of activity of G6PDH and 6PGDH compared to ME also suggest that
the major NADPH donors in trout liver are those involved in the pentose phosphate pathway and
that insulin acts as a stimulator of such a metabolic route (Novello et al., 1969).
Paradoxical regulation of β-oxidation Potential in Trout Liver by Insulin
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A paradoxical imbalance in the regulation of DNL and lipid oxidation pathways seems to
exist when insulin is infused. The CPT1 activity remained unchanged and even upregulated at
the molecular level, especially with the higher insulin dose. The absence of inhibition of CPT1
activity in our conditions could be due to the presence of long-chain n-3 fatty acids provided by
fish oil in the diet. Liver CPT1 activity is increased by n-3 fatty acids in mammals (Ide et al.,
2000). Surprisingly, we also found increased levels of HOAD activity in fed fish infused with
insulin. It was previously reported that high glucose levels in fish, both in vivo (ip injection;
Harmon et al., 1991) and in vitro (Harmon and Sheridan, 1992), stimulate lipolysis rates through
increased hepatic lipase activity. Moreover, in mammals increased levels of HOAD activity were
found in sand rats (Psammomys obesus) subjected to hyperglycemia and hyperinsulinemia
(Nakai et al., 1997). We therefore suggest that β-oxidation in trout liver is highly influenced by
diet composition (high levels of fish oil and carbohydrates), which could act as the major
regulator of CPT1 and HOAD activity, irrespective of the insulin dose.
Conclusions and perspective
Our findings indicate that DNL in rainbow trout is regulated by insulin, which increases
the 3 major enzymes involved in this pathway at molecular, protein, and enzyme activity levels.
This is further supported by the concomitant upregulation of some enzymes acting as NADPH
donors, especially those participating in the pentose phosphate pathway. The fact that insulin
also stimulates this pathway in high carbohydrate-fed rats (Nepokroeff et al., 1974) and in
hyperinsulinemic patients fed low-fat/high-carbohydrate diets (Schwarz et al., 2003), supports
the idea of a strongly conserved regulatory role of insulin in hepatic DNL. On the other hand,
although some studies in the 1970 to 1980s were contradictory concerning the role of insulin in
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high-carbohydrate-fed catfish (Warman III and Bottino, 1978; Machado et al., 1988), later
studies in vitro confirmed that insulin stimulates DNL in trout (Cowley and Sheridan, 1993).
This is relevant in carnivorous fish species fed high-carbohydrate diets, since their natural
carbohydrate intake is about 1%. Despite this apparent paradox, the incorporation of the excess
glucose from the diet into hepatic lipogenesis seems to be a common feature in this species
(Hung and Storebakken, 1994). In our study, part of the hypoglycemia observed in fish infused
with the lower insulin dose (data not shown) could then be due to this increased DNL potential.
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Figure legends
Figure 1. Effects of insulin infusion on liver Akt/PKB phosphorylation status in trout fed a high-
carbohydrate diet. Fish were implanted with pumps containing saline (control) or 2 insulin doses
(0.35 or 0.7 IU·kg–1·d-1) and then fed for 5 d. Gels were loaded with 20 µg total protein per lane.
Protein and phosphorylation levels were normalized to tissue β-tubulin levels and are indicated
as fold-change compared with the saline-treated group. Results are expressed as means ± SEM.
(n = 6).
Figure 2. Effects of insulin infusion on levels of ATP-citrate lyase (ACLY), acetyl-CoA
carboxylase (ACC), and fatty acid synthase (FAS) enzyme activity, protein levels, and mRNA
levels in livers of trout fed a high-carbohydrate diet. Gene expression was measured by realtime
PCR. Expression levels were normalized to elongation factor 1α (EF1α)-expressed transcripts
which did not change under the experimental conditions and are presented as fold-change against
the saline solution-treated group set at 1. Enzyme activity is expressed in mIU·mg-1 protein for
ACLY and µIU·mg-1 protein for ACC and FAS. Protein (20 µg per lane) and phosphorylation
levels were normalized to tissue β-tubulin levels and are indicated as fold-change compared to
the saline-treated group. Results are presented as means ± SEM. (n = 6).
Figure 3. Effects of insulin infusion on levels of glucose 6-phosphate dehydrogenase (G6PDH),
6-phosphogluconate dehydrogenase (6PGDH), malic enzyme (ME), and isocitrate
dehydrogenase (ICDH) enzyme activity and mRNA levels in livers of trout fed a high-
carbohydrate diet. Gene expression was measured by realtime PCR. Expression levels were
normalized to elongation factor 1α (EF1α)-expressed transcripts, which did not change under the
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experimental conditions and are presented as fold-change against the saline solution-treated
group set at 1. Enzyme activity is expressed in mIU·mg-1 protein. Results are presented as means
± SEM (n = 6).
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Table 1. Plasma glucose, tryglyceride, NEFA, and bovine insulin levels in rainbow trout fed a
high-carbohydrate diet and implanted with mini-osmotic pumps infusing saline alone (control)
or 2 insulin doses (0.35 or 0.7 IU·kg–1·d-1).
Parameter Saline Insulin 0.35 Insulin 0.7
Glucose (mM) 9.08 ± 0.42a 7.67 ± 0.42b 9.02 ± 0.44a
Tryglycerides (mM) 4.91 ± 0.56 6.36 ± 0.72 4.99 ± 0.40
NEFA (mEq·L-1) 0.126 ± 0.008a 0.107 ± 0.002b 0.097 ± 0.006b
Bovine insulin (ng·mL-1) no data 3.11 ± 0.34a 6.36 ± 0.65b
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Table 2. Hepatic enzyme activity and mRNA levels of β-oxidation-related enzymes in rainbow
trout fed a high-carbohydrate diet and implanted with mini-osmotic pumps infusing saline alone
(control) or 2 insulin doses (0.35 or 0.7 IU·kg–1·d-1).
Parameter Saline Insulin 0.35 Insulin 0.7
HOAD
Enzyme activity 46.61 ±
5.14a
82.43 ± 15.43b
(P = 0.048)
86.79 ± 13.32b
(P = 0.021)
mRNA levels 1.00 ± 0.26 1.98 ± 0.30
(P > 0.10)
1.20 ± 0.08
(P > 0.10)
CPT-1
Enzyme activity 8.21 ± 1.18 9.56 ± 0.50
(P > 0.10)
11.20 ± 2.26
(P > 0.10)
mRNA levels CPT1A 1.00 ± 0.20a 0.57 ± 0.11a
(P = 0.051)
1.64 ± 0.29b
(P = 0.025)
mRNA levels CPT1B 1.00 ± 0.25a 0.26 ± 0.05b
(P = 0.017)
0.37 ± 0.07b
(P = 0.025)
HOAD, 3-hydroxyacyl-CoA dehydrogenase; CPT-1, carnitin palmitoyltransferase 1. Enzyme activity units
(mIU) are defined as nmol of substrate converted to product, per min, at assay temperature, expressed/mg
protein. Expression levels were normalized to elongation factor 1α (EF1α)-expressed transcripts which did
not change under the experimental conditions and are presented in arbitrary units.
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Table 3. The P-value from one-way ANOVA of parameters measured in plasma and liver of high-carbohydrate-fed trout infused with saline solution alone or 2 insulin doses for 5 d.
Parameter P-value
Plasma
Glucose 0.044
Tryglycerides 0.738
NEFA 0.018
Bovine insulin 0.034
Liver mRNA
ACLY 0.010
FAS 0.030
ACC 0.248
G6PDH 0.039
6PGDH 0.007
ME 0.717
ICDH 0.046
HOAD 0.073
CPT1A 0.040
CPT1B 0.029
Liver proteins
Akt 0.941
ACLY 0.043
ACC 0.038
FAS 0.025
Liver activities
ACLY 0.136
FAS 0.042
ACC 0.015
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G6PDH 0.005
6PGDH 0.038
ME 0.217
ICDH 0.195
CPT1 0.390
HOAD 0.049
Non-esterified fatty acids (NEFA), ATP-citrate lyase (ACLY), fatty acid synthase (FAS), acetyl-CoA carboxylase (ACC), glucose 6-phosphate dehydrogenase (G6PDH), 6-phosphogluconate dehydrogenase (6PGDH), malic enzyme (ME), and isocitrate dehydrogenase (ICDH), 3-hydroxyacyl-CoA dehydrogenase (HOAD), carnitin palmitoyltransferase 1 (CPT-1), protein kinase B (Akt/PKB).
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Figure 1
Saline Insulin 0.35 Insulin 0.7
p-A
kt/t
ubulin
0.0
0.5
1.0
1.5
2.0
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Prote
in lev
els
0
1
2
3
a
a
b
a
a
b
a
a
b
mR
NA lev
els
0
1
2
3
a a
b
a
a
b
Figure 2
ACLY ACC FAS
ACLY
and A
CC
act
ivity
0
50
100
150
200
250
FAS a
ctiv
ity
0
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400
600
800
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1400Sal Ins 0.35Ins 0.7
aa
b
a
ab
b
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Figure 3
G6PDH 6PGDH ME ICDH
Enzy
me
activi
ty(m
U·m
g-1
pro
tein
)
0
20
40
60
80
100
120
140
160
180
ab
a
b
aba
b
aba
b
mRN
A lev
els
(fold
-induct
ion)
0
1
2
3
4
5
6
7Sal Ins 0.35 Ins 0.7
ab
a
b
b
a
b
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