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Am J Physiol Regul Integr Comp Physiol 290: R909-R915, 2006. First published December 8, 2005; doi:10.1152/ajpregu.00045.2005
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APPETITE, OBESITY, DIGESTION, AND METABOLISM

Different metabolic responses to central and peripheral injection of enterostatin

Ling Lin, MieJung Park, Matt Hulver, and David A. York

Pennington Biomedical Research Center, Baton Rouge, Louisiana

Submitted 21 January 2005 ; accepted in final form 4 June 2005


   ABSTRACT
TOP
 ABSTRACT
MATERIALS AND METHODS
 RESULTS
 DISCUSSION
 REFERENCES
 
Enterostatin, a pentapeptide cleaved from procolipase, suppresses fat intake after peripheral and central administration. Chronic treatment of rats with enterostatin decreases body weight and body fat. The effect was greater than could be accounted by the reduction in food intake alone. Hence, we have investigated the effect of enterostatin on energy metabolism. Male Sprague-Dawley rats adapted to a high-fat diet were implanted with lateral cerebral ventricular or amygdala cannulas. The metabolic effects were determined by indirect calorimetry. After habituation to the test cages, fasted rats were injected with either saline vehicle or enterostatin given either intraperitoneally (100 nmol) or intracerebroventricularly (1 nmol) or into specific brain regions [amygdala (0.01 nmol) or paraventricular nucleus (PVN) (0.1 nmol)]. Respiratory quotient (RQ) and energy expenditure were monitored over 2 h. Intraperitoneal enterostatin reduced RQ (saline: 0.81 ± 0.02 vs. enterostatin: 0.76 ± 0.01) and increased energy expenditure by 44%. Intracerebroventricular enterostatin increased the energy expenditure without any effects on RQ, whereas PVN enterostatin increased metabolic rate, while preventing the increase in RQ observed in the control animals. In contrast, neither RQ nor energy expenditure was altered after enterostatin was injected into the amygdala. Enterostatin activated AMP-activated protein kinase in primary cultures of human myocytes in a dose- and time-dependent manner and increased the rate of fatty acid beta-oxidation. These findings suggest that enterostatin regulates energy expenditure and substrate partitioning through both peripheral and central effects.

amygdala; indirect calorimetric system; respiratory quotient; adenosine 5'-diphosphate-active protein kinase; myocytes; beta-oxidation

ENTEROSTATIN, A PENTAPEPTIDE, is a cleavage product of pancreatic procolipase released during activation of the cofactor in the intestine after the ingestion of dietary fat (8). Procolipase is also expressed in the stomach, duodenal mucosa, and in specific brain regions (20, 36, 47, 52). Enterostatin acts as an early satiety factor to regulate energy intake, specifically the intake of dietary fat (7, 9, 22). Exogenous administration of enterostatin selectively suppressed fat intake in rats after both peripheral and central administration (18, 19, 21, 22, 24, 27, 29, 46). The peripheral site of action is in the gastroduodenal region, and this response is mediated through the afferent vagus (18). Central action sites include the paraventricular nucleus (PVN) in the hypothalamus and the amygdala region of the limbic system, with maximum inhibitory effect being observed in the central nucleus of amygdala (26, 27). The central pathway activated by enterostatin includes opioid, serotonin, and CCK components (23, 25, 38).

Maintenance of energy balance requires a balance between energy intake and expenditure. The regulation of these two limbs of energy balance is physiologically linked, through hypothalamic and other central nervous system (CNS) circuits (10, 48). Most of the peptides that regulate energy intake also affect energy expenditure (EE), such as neuropeptide Y (NPY), leptin, melanin-concentrating hormone (MCH), corticotropin releasing hormone (CRH) (4, 5, 12, 30, 31, 49). Obesity may result from either increased feeding and/or decreased EE, as exemplified by the obesity that results from defects in either leptin signaling or the melanocortin pathway (3, 11).

Although there are numerous reports to support the effect of enterostatin on feeding, little is known about the metabolic effects of enterostatin. The possible effects on EE or energy substrate utilization are suggested by several lines of evidence. First, chronic infusion of enterostatin intraperitoneally or intracerebroventricularly caused weight and body fat loss that seemed to be greater than could be accounted for the reduction of food intake (19, 35); second, enterostatin treatment increases sympathetic outflow to brown adipose tissue (34) and enhances uncoupling protein 1 mRNA levels and heat production (42); third, acute and chronic administration of enterostatin increases the serum corticosterone levels (19, 35), which is critical to the EEs (12). Moreover, an in vitro study showed that enterostatin stimulated oxygen consumption in INS-1 cells (2). The present study was designed to characterize the effects of acute peripheral and central injection of enterostatin on EE in rats by using indirect calorimetry. In addition, we have demonstrated a direct effect of enterostatin on muscle to activate AMP-activated protein kinase (AMPK) and beta-oxidation of fatty acids. AMPK is now recognized to have a central role in regulating the balance between anabolic and catabolic pathways in peripheral tissues (13, 43).


   MATERIALS AND METHODS
TOP
 ABSTRACT
 MATERIALS AND METHODS
RESULTS
 DISCUSSION
 REFERENCES
 
Peptides and antibodies. Enterostatin was synthesized by solid-phase chemistry, purified by HPLC, and estimated to be of greater than 90% purity by the Core Laboratory of Louisiana State University Medical Center (New Orleans, LA). Antibodies against phospho-AMPK and AMPK were purchased from Upstate Biotechnology (Lake Placid, NY). beta-Actin antibody was obtained from Abcam (Cambridge, UK).

Animals and diet. Forty-eight male Harlan Sprague-Dawley rats (300–400 g body wt, Harlan Sprague-Dawley, Indianapolis, IN) were used in the current study. They were housed individually in acrylic cages in a temperature-controlled room (22–23°C) with a 12:12-h light-dark cycle (lights on at 0700) and with free access to an automatic watering system. The rats were adapted to a high-fat diet (4.78 kcal/g, 56% of energy as fat) ad libitum for a minimum of 2 wk. The composition of the diet has been described elsewhere (19). The experimental procedures and protocols were reviewed and approved by the Institutional Animal Care and Use Committee.

Surgery. Animals were anesthetized with pentobarbital sodium (Nembutal; 0.1 ml/100 g body wt ip). Each rat was stereotaxically implanted with one unilateral cannula. A stainless steel cannula was aimed to the lateral ventricle, PVN, or central nucleus of the amygdala. The coordinates (AP/L/DV to bregma) were lateral ventricle: –1.4/–0.8/–4.0 mm; PVN: –1.9/–0.4/6.0 mm; amygdala: –2.4/–3.8/–6.0 mm (40). Each cannula was secured in place with three anchor screws and dental acrylic and occluded with a stylet. The injectors for PVN and amygdala were designed to projected 2 mm beyond the guide cannula tip. The animals were returned to the home cages after recovery from the anesthesia and maintained on the diet. Experiments began after rats had regained their preoperative weight (about 10 days).

Peptide injections. Enterostatin was dissolved in saline (0.9% wt/vol) and given as a single injection at doses of 120, 1, 0.1 or 0.01 nmol ip, icv, PVN, or amygdala, respectively. All of the above doses were experimentally shown previously to have maximum inhibitory effect on feeding (22, 27, 37). The rats assigned as a vehicle control group were given saline in a volume of 0.1 ml for ip, 5 µl for icv, 0.1 µl for PVN or amygdala.

Apparatus. An open circuit calorimeter (Oxymax, Columbus Instruments, Columbus, OH) was used to monitor oxygen and carbon dioxide gas fractions at both the inlet and output ports to the test chambers, which consisted of 12 enclosed acrylic chambers similar to the rat's home cage. The airflow was 1.0 l/min. Air from each chamber was sampled and analyzed for 35 s in every 7 min. The gas fraction and flow measurements were used to compute oxygen consumption (VO2), carbon dioxide production (VCO2), respiratory quotient (RQ) and EE. All testing was conducted during the light cycle from 1000 to 1500, as the physical activity of the rats was minimum at this time of the day. The animals were habituated to the chambers for 5 h/day for 3 days before testing. On the test days, the rats were assigned to saline or enterostatin treatment groups, according to their body weight and placed in the chambers. Once RQ had reached stable values, the rats were removed from the chambers and injected with either vehicle or enterostatin, as described above; then they were immediately returned to the chambers. The RQ was allowed to reach equilibrium again (~21 min) before measurements were taken. Food and water were not available during measurement of EE (5, 12). At the conclusion of the experiments, rats were killed, and brain cannula placements were determined by histology and comparison to the rat brain atlas of Paxinos and Watson (40).

Immunoblotting. Whole cell lysates were made by sonication in lysis buffer (1% Triton X-100, 50 mM KCl, 25 mM HEPES, pH 7.8, 10 µg/ml leupeptin, 20 µg/ml aprotinin, 125 µM dithiothreitol, 1 mM phenylmethylsulfonyl fluoride, 1 mM sodium orthovanadate). Samples (100 µg of total protein) in 50 µl of reducing sample buffer were boiled for 5 min and resolved on 10% mini-SDS-PAGE for 90 min at 100 v. The contents of the gel were transferred onto polyvinylidene difluoride membrane (Roche, Indianapolis, IN) at 50 v for 120 min. The membrane was preblotted in milk buffer [5% nonfat milk in Tris-buffered saline-Tween (TBST); 10 mM Tris·HCl (pH 7.5), 150 mM NaCl, 0.05% Tween 20] for 120 min and then immunoblotted with primary antibody for 18 h followed by secondary antibody for 30 min after washing with TBST. Horseradish peroxidase-conjugated secondary antibody (Santa Cruz Biotechnology, Santa Cruz, CA) was used in conjunction with chemiluminescence reagent (ECL detection kit, Amersham Pharmacia, Buckinghamshire, UK, or visualizer from Upstate Biotechnology).

Fatty acid oxidation in human primary muscle cell cultures. Human skeletal muscle cells were cultured as previously described (32, 33). Briefly, muscle samples were obtained from the vastus lateralis muscle by needle biopsy, and satellite cells were isolated by trypsin digestion (14). Cells were grown to confluency on type I collagen-coated T25 flask at 37°C in a humidified atmosphere of 5% CO2 in DMEM supplemented with 10% FBS, 0.5 mg/ml BSA, 0.5 mg/ml fetuin, 20 ng/ml human epidermal growth factor, 0.39 µg/ml dexamethasone, and 50 µg/ml gentamicin/amphotericin B. After reaching ~90% confluency, myoblasts were subcultured onto a six-well, type I collagen-coated plates at densities of 96 x 103 cells per well. When cells reached 90% confluency, differentiation was induced by changing to low-serum differentiation media consisting of 2% heat-inactivated horse serum, 0.5 mg/ml BSA, 0.5 mg/ml fetuin, and 50 µg/ml gentamicin/amphotericin B.

Fatty acid oxidation was measured on the 7th day of differentiation under the following conditions: control, 0.01 µM enterostatin, and 1.0 µM enterostatin. Briefly, cells were incubated at 37°C in sealed six-well plates, containing 2.0 ml of serum-free differentiation media plus 12.5 mmol/l HEPES, 0.2% BSA, 1.0 mmol/l carnitine, 100 µmol/l oleate, 50 µg/ml gentamicin, and 1.0 µCi/ml [14C]oleate (NEN, Boston, MA). After 3 h, incubation media were sampled and assayed for 14C-labeled CO2 and acid-soluble metabolites (ASM), as previously described (15, 17). The cells were placed on ice, washed twice with ice-cold PBS, and scraped into a 1.5-ml Eppendorf tube in two additions of 0.30 ml 0.05% SDS lysis buffer. Lysates were stored at –80°C for determination of protein content. Total fatty acid oxidation is denoted as CO2 + ASM production in nmol·mg–1 protein·h–1.

Data analysis. RQ and EE data are expressed as means ± SE with six rats in each treatment group. EE was derived from the computer-generated data and normalized by body weight across subjects as J·h–1·100 g body wt–1 (1, 28). The difference between the treatments was analyzed by ANOVA with repeated measures, and post hoc tests were performed by using the Bonferroni correction.


   RESULTS
TOP
 ABSTRACT
 MATERIALS AND METHODS
 RESULTS
DISCUSSION
 REFERENCES
 
Verification of the cannula placements. Figure 1 shows an example of histological verification of the positions of the cannula. The tract of the unilateral cannula in the rat coronal sections terminates directly above either the PVN (Fig. 1A) or the central nucleus of the amygdala (Fig. 1B), compared with the schematic illustrations of rat brain (Fig. 1, C and D).


Figure 1
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  		Fig. 1. Photography of the coronal sections of rat brain showing the cannula tract in the paraventricular nucleus (PVN; A) and central nucleus of amygdala (CeA) (B). The inlets (A and B) are the pictures taken under a microscope with x10 magnification. Schematic illustrations of those sites (C: PVN; D: central nucleus of the amygdala) are adapted from Paxinos and Watson (40). Open arrows show PVN, and solid arrows show the amygdala.

 
Changes of RQ after the injection of enterostatin. The time course of the effects of enterostatin on RQ after injection into intraperitoneal, intracerebroventricular, PVN, or amygdala sites is shown in Fig. 2. Rats receiving a peripheral injection of enterostatin (120 nmol) (Fig. 2A) had a decreased RQ compared with vehicle controls after 35 min (saline 0.80 vs. enterostatin 0.75). ANOVA showed a significant difference over the observed period with intraperitoneal enterostatin treatment [main treatment effects: F(1,10)=19.13, P < 0.001]. However, this resulted mainly from an increase in RQ in the control animals rather than a decrease in RQ in the enterostatin-treated rats. A similar effect was also seen after injection of enterostatin (0.1 nmol) into the PVN (saline 0.88 vs. enterostatin 0.82 at 35 min). This effect was statistically significant [main treatment effects: F(1,10) = 5.28, P < 0.05]. No effects of treatments were observed after intracerebroventricular [main treatment effects: F(1,10) = 0.759, P = 0.404] or amygdala [main treatment effects: F(1,10) = 1.908, P = 0.197] injections (Fig. 2, B and D).


Figure 2
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  		Fig. 2. Respiratory quotient (RQ) after the injection of either saline or enterostatin through intraperitoneal (A), intracerebroventricular (B), PVN (C) and central nucleus of amygdala (D) in rats with a chronic cannula aimed to the corresponding site (n = 6 in saline or enterostatin treatment group). The data were collected every 7 min. E: average RQ over the testing period. Data are expressed as means ± SE for 6 rats in each group. *P < 0.05, **P < 0.001 compared with respective saline group.

 
In Fig. 2E, RQ is expressed as the average over the 2-h testing period. There was a significant decrease in RQ after intraperitoneal enterostatin treatment (saline: 0.790 ± 0.004 vs. enterostatin: 0.761 ± 0.003, P < 0.001) and after PVN treatment (saline: 0.862 ± 0.003 vs. enterostatin: 0.841 ± 0.002, P < 0.001). No effects were observed with enterostatin injected intracerebroventricularly or into the amygdala.

Effects of enterostatin on EE. As shown in Fig. 3, A and E, intraperitoneal enterostatin increased EE by 32%, the effect being observed within 14 min (saline 2,141.7 ± 51.5 vs. enterostatin 2,837.9 ± 56.1 J·h–1·/100 g body wt–1) and lasting throughout the whole test period (126 min) [main treatment effects: F(1,10)= 38.36, P < 0.0001]. Intracerebroventricular injections reduced metabolic rates, but enterostatin-treated rats maintained a higher EE (20% at 21 min) than saline vehicle-treated rats (Fig. 3, B and E). The main treatment effect of intracerebroventricular enterostatin was significant [F(1,10) = 6.584, P < 0.05]. PVN injection of enterostatin (Fig. 3, C and E) increased EE by ~25% overall with a maximum 35% increase at 56 min [saline: 2,604.3 ± 105.9 vs. PVN enterostatin: 3,527.7 ± 211.5 J·h–1·100 g body wt–1, F(1,10)=5.537, P < 0.05]. Injection of enterostatin into the amygdala had no effect on EE [F(1,10) = 0.035, P = 0.856].


Figure 3
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  		Fig. 3. Energy expenditure (EE) after the injection of saline or enterostatin through different routes (see Fig. 2). The data are expressed as J·h–1·100 g body wt–1 of rat. E: average energy expenditure over 2-h testing period. Data are expressed as means ± SE for 6 rats in each group. *P < 0.05, **P < 0.001 compared with respective saline group.

 
Effect of enterostatin on AMPK and beta-oxidation in primary myocyte cultures. Enterostatin-activated AMPK in primary myocytes in a time- and dose-dependent manner (Fig. 4, A and B). Maximum levels of phospho-AMPK were observed at 15-min incubation time with enterostatin, and the strongest activation was observed with 10 nM enterostatin but was lower at higher concentrations of enterostatin. Likewise, the fourfold increase in fatty acid oxidation (Fig. 4C) was observed at 10 nM enterostatin but not at the higher dose of 1 µM.


Figure 4
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  		Fig. 4. Enterostatin activation of AMP kinase (AMPK) and fatty acid oxidation in primary cultures of human myocytes. A: dose response to enterostatin. B: time course of the response to 1 µM enterostatin. C: fatty acid oxidation in response to enterostatin. The values for fatty acid oxidation represent the means ± SE for 12 replicates.

 

   DISCUSSION
TOP
 ABSTRACT
 MATERIALS AND METHODS
 RESULTS
 DISCUSSION
REFERENCES
 
This study reports new observations that the anorectic peptide enterostatin regulates EE and substrate oxidation after both peripheral and central administration. Injection of enterostatin intraperitoneally and into the PVN reduced RQ, indicating an increased fat utilization, and also increased EE. In contrast, the finding that enterostatin injections into the central nucleus of amygdala did not affect RQ or EE suggests that the regulation of EE and food intake by enterostatin involves different neural circuits. Further, the studies with primary myocyte cultures suggest that enterostatin has a direct effect on muscle to enhance fatty acid oxidation.

Energy balance is determined by food intake and EE. Increasing the food intake and/or decreasing the EE will lead to obesity (41). Enterostatin, like many other gut peptides, appears to have both peripheral and central effects (22, 37). The central actions probably do not relate to uptake of circulating enterostatin into the CNS, as recent data, using immunohistochemistry and RT PCR, have provided evidence for the synthesis of procolipase and release of enterostatin in specific brain regions (20). Most of the peptides that regulate food intake have also been shown to have an impact on EE. These dual effects have been well demonstrated for NPY, CRH, leptin, {alpha}-MSH, and galanin (4, 5, 12, 30, 31, 49, 53). In this light, it is not surprising that enterostatin, an early satiety factor, also has effects on EE, as found in this study.

Another characteristic of most neuropeptides that affect feeding is the opposing effects on food intake and EE. Thus the anorectic peptides (for example, NPY, agouti-related protein) provoke food intake and reduce EE, whereas the catabolic peptides (for example, {alpha}-MSH, CCK) decrease food intake, while enhancing sympathetically mediated EE. Enterostatin, likewise, affects both sides of the energy balance equation, suppressing dietary fat intake, while positively increasing fat utilization (decrease of RQ) and EE. These observations are consistent with our previous findings that chronic administration of enterostatin, both peripherally and centrally, decreases fat pad weight and body weight (19).

The hypothalamus plays an important role in the regulation of feeding and EE. Multiple subregions are involved in EE, including the arcuate PVN, ventromedial hypothalamus, and lateral hypothalamus (5, 6, 32, 44). The circuitry regulating food intake has been described in detail in recent years (45), but there is less insight into the circuits regulating EE. However, studies with NPY suggest a separation of the two control circuits. For example, the perifornical hypothalamus appears to mediate only the feeding-stimulatory actions of NPY, whereas PVN regulates metabolic processes (5). The current study had a similar observation that enterostatin into the PVN changes both RQ and EE, but neither RQ nor EE was affected by injection of enterostatin into the amygdala. We previously demonstrated that the amygdala is the most sensitive site for induction of enterostatin feeding response within the brain (26, 27) and have described the circuits that are activated in response to amygdala enterostatin. Together with other recent reports that the amygdala is critical for ingestion of dietary fat (16, 50), the evidence suggests that the amygdala may be the center for the regulation of fat intake by enterostatin but that enterostatin regulation of EE may be initiated by a circuit activated in the PVN.

In this study, we only used a single dose of enterostatin for each route of administration. It may be argued that a dose-response curve might identify effects of enterostatin at higher doses. However, the doses we chose have been previously demonstrated to have maximal effects on inhibition of feeding (22, 27, 37). The absence of any effects on EE, using the maximal amygdala dose, and the presence of effects in the PVN provide us with confidence in our conclusion that the amygdala is a major site for enterostatin regulation of dietary fat intake, whereas the PVN is a major site for enterostatin regulation of EE. It is unlikely that the effects of central enterostatin on EE relate to the inducement of illness, as previous studies on feeding behavior have shown that enterostatin does not induce a conditioned taste aversion (26).

AMPK is thought to play a central role in the regulation of nutrient partitioning and the control of anabolic and catabolic pathways. Activation of AMPK by phosphorylation has been associated with an increase in fatty acid oxidation and glucose transport in muscle and a decrease in fatty acid synthesis and gluconeogenesis in liver (43, 51). In the current studies, using primary human myocyte cultures, we showed that enterostatin had a direct effect on myocytes to activate AMPK and increase fatty acid oxidation. This occurred in a dose-dependent manner with maximum activation around 10 nM enterostatin. Previous studies with enterostatin have also shown a U-shaped dose-response curve on food intake (18) and on receptor binding (39). The amino acid sequence of enterostatin is identical in rat and man, Ala-Pro-Gly-Pro-Arg, so the effect of enterostatin to increase fatty acid oxidation in human myocytes is suggestive that a similar response may be evident in rodent muscle. Certainly, these in vitro culture data are consistent with the in vivo data reported here that intraperitoneal enterostatin increased EE and decreased RQ, that is, increased fatty acid oxidation. Our results suggest that this stimulation of fatty acid oxidation in muscle was, at least, partly responsible for this effect. Whether enterostatin also increases fatty oxidation in other tissues such as liver, is not known at this time.

In conclusion, the experiments reported here provide convincing data that enterostatin has metabolic effects in addition to its effects on feeding behavior. The interpretation of the data on RQ is difficult. The RQ of enterostatin-treated rats was significantly reduced compared with vehicle-treated rats after intraperitoneal and PVN administration. However, in both cases, the difference mainly resulted from an increase in RQ in the control vehicle-treated rats. Because these measurements were made in the absence of food, it is possible that the handling of rats was associated with a sympathetically mediated increase in glycogenolysis and subsequent increase in carbohydrate availability and oxidation that was not observed in enterostatin-treated rats or was counteracted by the promotion of lipolysis and fat oxidation. Likewise, it is not clear why the RQ levels of all rats with cannulas directed at the PVN was higher, around 0.85, despite the sole access to a high-fat diet. It is possible again that the indwelling cannulas themselves caused an activation of the autonomic nervous system that led to enhanced availability of carbohydrates for oxidation.

The mechanism through which enterostatin increases EE is probably twofold. First, it increases sympathetic drive to brown adipose tissue, uncoupling protein 1 transcription, and thermogenesis (42) and would be expected to increase lipolysis and fatty acid oxidation. Second, the demonstration that membrane-located beta-subunit of F1-ATP synthase is the enterostatin receptor (39) and that enterostatin reduces cell ATP levels suggests that all cells that have enterostatin receptors will also increase ATP turnover and heat production. Such a change in ATP levels is likely responsible for the activation of AMPK and the stimulation of muscle fatty acid oxidation that we have reported in this study.


   FOOTNOTES
 

Address for reprint requests and other correspondence: David A. York, Pennington Biomedical Research Ctr., 6400 Perkins Rd., Baton Rouge, LA 70808 (e-mail: yorkda{at}pbrc.edu)

The costs of publication of this article were defrayed in part by the payment of page charges. The article must therefore be hereby marked "advertisement" in accordance with 18 U.S.C. Section 1734 solely to indicate this fact.


   REFERENCES
TOP
 ABSTRACT
 MATERIALS AND METHODS
 RESULTS
 DISCUSSION
 REFERENCES
 

  1. Atrens DM, Siviy SM, Holmes LJ, Solowij N, and Jirasek M. Hypothalamic modulation of thermogenesis and energy substrate utilization. Brain Res Bull 18: 303–308, 1987.[CrossRef][Web of Science][Medline]
  2. Berger K, Sivars U, Winzell MS, Johansson P, Hellman U, Rippe C, and Erlanson-Albertsson C. Mitochondrial ATP synthase–a possible target protein in the regulation of energy metabolism in vitro and in vivo. Nutr Neurosci 5: 201–210, 2002.[CrossRef][Web of Science][Medline]
  3. Butler AA and Cone RD. The melanocortin receptors: lessons from knockout models. Neuropeptides 36: 77–84, 2002.[CrossRef][Web of Science][Medline]
  4. Chen AS, Metzger JM, Trumbauer ME, Guan XM, Yu H, Frazier EG, Marsh DJ, Forrest MJ, Gopal-Truter S, Fisher J, Camacho RE, Strack AM, Mellin TN, MacIntyre DE, Chen HY, and Van der Ploeg LH. Role of the melanocortin-4 receptor in metabolic rate and food intake in mice. Transgenic Res 9: 145–154, 2000.[CrossRef][Web of Science][Medline]
  5. Currie PJ and Coscina DV. Regional hypothalamic differences in neuropeptide Y-induced feeding and energy substrate utilization. Brain Res 737: 238–242, 1996.[CrossRef][Web of Science][Medline]
  6. Currie PJ, Coscina DV, Bishop C, Coiro CD, Koob GF, Rivier J, and Vale W. Hypothalamic paraventricular nucleus injections of urocortin alter food intake and respiratory quotient. Brain Res 916: 222–228, 2001.[CrossRef][Web of Science][Medline]
  7. Erlanson-Albertsson C, Mei J, Okada S, York D, and Bray GA. Pancreatic procolipase propeptide, enterostatin, specifically inhibits fat intake. Physiol Behav 49: 1191–1194, 1991.[CrossRef][Medline]
  8. Erlanson-Albertsson C, Westrom B, Pierzynowski S, Karlsson S, and Ahren B. Pancreatic procolipase activation peptide-enterostatin-inhibits pancreatic enzyme secretion in the pig. Pancreas 6: 619–624, 1991.[Web of Science][Medline]
  9. Erlanson-Albertsson C and York D. Enterostatin–a peptide regulating fat intake. Obes Res 5: 360–372, 1997.[Web of Science][Medline]
  10. Flier JS. Obesity wars: molecular progress confronts an expanding epidemic. Cell 116: 337–350, 2004.[CrossRef][Web of Science][Medline]
  11. Friedman JM and Halaas JL. Leptin and the regulation of body weight in mammals. Nature 395: 763–770, 1998.[CrossRef][Medline]
  12. Hamelink CR, Currie PJ, Chambers JW, Castonguay TW, and Coscina DV. Corticosterone-responsive and -unresponsive metabolic characteristics of adrenalectomized rats. Am J Physiol Regul Integr Comp Physiol 267: R799–R804, 1994.[Abstract/Free Full Text]
  13. Hardie DG. The AMP-activated protein kinase pathway: new players upstream and downstream. J Cell Sci 117: 5479–5487, 2004.[Abstract/Free Full Text]
  14. Henry RR, Ciaraldi TP, Abrams-Carter L, Mudaliar S, Park KS, and Nikoulina SE. Glycogen synthase activity is reduced in cultured skeletal muscle cells of non-insulin-dependent diabetes mellitus subjects. Biochemical and molecular mechanisms. J Clin Invest 98: 1231–1236, 1996.[Web of Science][Medline]
  15. Hulver MW, Berggren JR, Cortright RN, Dudek RW, Thompson RP, Pories WJ, MacDonald KG, Cline GW, Shulman GI, Dohm GL, and Houmard JA. Skeletal muscle lipid metabolism with obesity. Am J Physiol Endocrinol Metab 284: E741–E747, 2003.[Abstract/Free Full Text]
  16. Kelley AE. Ventral striatal control of appetitive motivation: role in ingestive behavior and reward-related learning. Neurosci Biobehav Rev 27: 765–776, 2004.[CrossRef][Web of Science][Medline]
  17. Kim JY, Hickner RC, Cortright RL, Dohm GL, and Houmard JA. Lipid oxidation is reduced in obese human skeletal muscle. Am J Physiol Endocrinol Metab 279: E1039–E1044, 2000.[Abstract/Free Full Text]
  18. Lin L, Bray G, and York DA. Enterostatin suppresses food intake in rats after near-celiac and intracarotid arterial injection. Am J Physiol Regul Integr Comp Physiol 278: R1346–R1351, 2000.[Abstract/Free Full Text]
  19. Lin L, Chen J, and York DA. Chronic ICV enterostatin preferentially reduced fat intake and lowered body weight. Peptides 18: 657–661, 1997.[CrossRef][Web of Science][Medline]
  20. Lin L, Braymer HD, and York DA. Procolipase gene and enterostatin expression in the rat brain (Abstract). FASEB J: A783, 2002.
  21. Lin L, McClanahan S, York DA, and Bray GA. The peptide enterostatin may produce early satiety. Physiol Behav 53: 789–794, 1993.[CrossRef][Medline]
  22. Lin L, Okada S, York DA, and Bray GA. Structural requirements for the biological activity of enterostatin. Peptides 15: 849–854, 1994.[CrossRef][Web of Science][Medline]
  23. Lin L, Thomas SR, Kilroy G, Schwartz GJ, and York DA. Enterostatin inhibition of dietary fat intake is dependent on CCK-A receptors. Am J Physiol Regul Integr Comp Physiol 285: R321–R328, 2003.[Abstract/Free Full Text]
  24. Lin L, Umahara M, York DA, and Bray GA. Beta-casomorphins stimulate and enterostatin inhibits the intake of dietary fat in rats. Peptides 19: 325–331, 1998.[CrossRef][Web of Science][Medline]
  25. Lin L and York DA. 5HT1B receptors modulate the feeding inhibitory effects of enterostatin. Brain Res 1062: 26–31, 2005.[CrossRef][Web of Science][Medline]
  26. Lin L and York DA. Changes in the microstructure of feeding after administration of enterostatin into the paraventricular nucleus and the amygdala. Peptides 19: 557–562, 1998.[CrossRef][Web of Science][Medline]
  27. Lin L and York DA. Enterostatin actions in the amygdala and PVN to suppress feeding in the rat. Peptides 18: 1341–1347, 1997.[CrossRef][Web of Science][Medline]
  28. McGregor IS and Lee AM. Metabolic changes associated with ingestion of different macronutrients and different meal sizes in rats. Physiol Behav 57: 277–286, 1995.[CrossRef][Medline]
  29. Mei J and Erlanson-Albertsson C. Role of intraduodenally administered enterostatin in rats: inhibition of food. Obes Res 4: 161–165, 1996.[Web of Science][Medline]
  30. Menendez JA, McGregor IS, Healey PA, Atrens DM, and Leibowitz SF. Metabolic effects of neuropeptide Y injections into the paraventricular nucleus of the hypothalamus. Brain Res 516: 8–14, 1990.[CrossRef][Web of Science][Medline]
  31. Mistry AM, Swick AG, and Romsos DR. Leptin rapidly lowers food intake and elevates metabolic rates in lean and ob/ob mice. J Nutr 127: 2065–2072, 1997.[Abstract/Free Full Text]
  32. Muoio DM, MacLean PS, Lang DB, Li S, Houmard JA, Way JM, Winegar DA, Corton JC, Dohm GL, and Kraus WE. Fatty acid homeostasis and induction of lipid regulatory genes in skeletal muscles of peroxisome proliferator-activated receptor (PPAR) alpha knock-out mice. Evidence for compensatory regulation by PPARdelta. J Biol Chem 277: 26089–26097, 2002.[Abstract/Free Full Text]
  33. Muoio DM, Way JM, Tanner CJ, Winegar DA, Kliewer SA, Houmard JA, Kraus WE, and Dohm GL. Peroxisome proliferator-activated receptor-{alpha} regulates fatty acid utilization in primary human skeletal muscle cells. Diabetes 51: 901–909, 2002.[Abstract/Free Full Text]
  34. Nagase H, Bray GA, and York DA. Effect of galanin and enterostatin on sympathetic nerve activity to interscapular brown adipose tissue. Brain Res 709: 44–50, 1996.[CrossRef][Web of Science][Medline]
  35. Okada S, Lin L, York DA, and Bray GA. Chronic effects of intracerebral ventricular enterostatin in Osborne-Mendel rats fed a high-fat diet. Physiol Behav 54: 325–329, 1993.[CrossRef][Medline]
  36. Okada S, York DA, and Bray GA. Procolipase mRNA: tissue localization and effects of diet and adrenalectomy. Biochem J 292: 787–789, 1993.
  37. Okada S, York DA, Bray GA, Mei J, and Erlanson-Albertsson C. Differential inhibition of fat intake in two strains of rat by the peptide enterostatin. Am J Physiol Regul Integr Comp Physiol 262: R1111–R1116, 1992.[Abstract/Free Full Text]
  38. Ookuma K, Barton C, York DA, and Bray GA. Effect of enterostatin and kappa-opioids on macronutrient selection and consumption. Peptides 18: 785–791, 1997.[CrossRef][Web of Science][Medline]
  39. Park MJ, Lin L, Thomas SR, Braymer DH, and York DA. The F1-ATPase Beta subunit is the putative enterostatin receptor. Peptides 25: 2127–2133, 2004.[CrossRef][Web of Science][Medline]
  40. Paxinos G and Watson C. The Rat Brain in Stereotaxic Coordinates. Sydney, Australia: Academic Press, 1982.
  41. Prentice A and Jebb S. Energy intake/physical activity interactions in the homeostasis of body weight regulation. Nutr Rev 62: S98–S104, 2004.[CrossRef][Web of Science][Medline]
  42. Rippe C, Berger K, Boiers C, Ricquier D, and Erlanson-Albertsson C. Effect of high-fat diet, surrounding temperature, and enterostatin on uncoupling protein gene expression. Am J Physiol Endocrinol Metab 279: E293–E300, 2000.[Abstract/Free Full Text]
  43. Ruderman N and Prentki M. AMP kinase and malonyl CoA: targets for the therapy of the metabolic syndrome. Nat Rev Drug Discov 3: 340–351, 2004.[CrossRef][Web of Science][Medline]
  44. Ruffin MP, Caulliez R, and Nicolaidis S. Parallel metabolic and feeding responses to lateral hypothalamic stimulation. Brain Res 700: 121–128, 1995.[CrossRef][Web of Science][Medline]
  45. Schwartz MW, Woods SC, Porte D Jr, Seeley RJ, and Baskin DG. Central nervous system control of food intake. Nature 404: 661–671, 2000.[Medline]
  46. Sorhede M, Mei J, and Erlanson-Albertsson C. Enterostatin: a gut-brain peptide regulating fat intake in rat. J Physiol Paris 87: 273–275, 1993.[CrossRef][Web of Science][Medline]
  47. Sorhede M, Mulder H, Mei J, Sundler F, and Erlanson-Albertsson C. Procolipase is produced in the rat stomach–a novel source of enterostatin. Biochim Biophys Acta 1301: 207–212, 1996.[Medline]
  48. Spiegelman BM and Flier JS. Obesity and the regulation of energy balance. Cell 104: 531–543, 2001.[CrossRef][Web of Science][Medline]
  49. Wang T, Hartzell DL, Rose BS, Flatt WP, Hulsey MG, Menon NK, Makula RA, and Baile CA. Metabolic responses to intracerebroventricular leptin and restricted feeding. Physiol Behav 65: 839–848, 1999.[CrossRef][Medline]
  50. Will MJ, Franzblau EB, and Kelley AE. The amygdala is critical for opioid-mediated binge eating of fat. Neuroreport 15: 1857–1860, 2004.[CrossRef][Web of Science][Medline]
  51. Winder WW and Hardie DG. AMP-activated protein kinase, a metabolic master switch: possible role in type 2 diabetes. Am J Physiol Endocrinol Metab 277: E1–E10, 1999.[Abstract/Free Full Text]
  52. Winzell MS, Lowe ME, and Erlanson-Albertsson C. Rat gastric procolipase: sequence, expression, and secretion during high-fat feeding. Gastroenterology 115: 1179–1185, 1998.[CrossRef][Web of Science][Medline]
  53. Yamashita J, Onai T, York DA, and Bray GA. Relationship between food intake and metabolic rate in rats treated with beta-adrenoceptor agonists. Int J Obes Relat Metab Disord 18: 429–433, 1994.[Web of Science][Medline]




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