Abstract
Preproghrelin, a gut/brain peptide, plays an important role in the regulation of food intake and energy homeostasis in teleost and mammals. In the present study, we obtained the full-length preproghrelin cDNA in Chinese perch. The preproghrelin messenger RNA (mRNA) tissue expression showed that level was much higher in stomach and pituitary than in other tissues. The fasting study showed, after gastric emptying (3–6 h), short-term fasting (6–12 h) increased preproghrelin expression in the stomach. While in the pituitary, fasting reduced preproghrelin expression at 1, 3, 12, and 48 h, presenting state fluctuation of self-adjustment. The temperature study showed that the mRNA expression of preproghrelin was the highest in the brain at 26 °C and highest in the stomach at 32 °C, respectively, with different optimum temperature in these two tissues, reflecting spatiotemporal differences of regulation by central nervous system and peripheral organs. The photoperiod study showed that normal light (11 h of lightness and 13 h of darkness) led to highest preproghrelin expression, both in the brain and in the stomach, than continuous light or continuous dark, proving food intake is adapted to natural photoperiod or normal light in this study. These results all indicated that tissue-specific preproghrelin expression of Chinese perch could be significantly affected by environmental factors. Short-term fasting of 6 h after gastric emptying, 26 °C, and normal light led to higher preproghrelin expression, which indicated potential appetite increase in Chinese perch.
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Introduction
Food intake in vertebrates is regulated through a complex interaction of several neuroendocrine factors derived from both the central nervous system and peripheral organs (Volkoff et al. 2009). Preproghrelin, a gut/brain peptide, was originally purified and characterized in the stomach of rats and humans, and identified as the first endogenous ligand of the growth hormone secretagogue receptor (GHSR). Central or peripheral administration of preproghrelin stimulates the release of growth hormone (GH) (Kojima et al. 1999; Wren et al. 2000), promotes food intake, and increases body weight gain in rats (Wren et al. 2000; Nakazato et al. 2001). Therefore, preproghrelin is considered the third polypeptide that regulates GH secretion in addition to growth hormone releasing hormone and somatostatin (Wang et al. 2002). In fish, preproghrelin is also considered to regulate somatic growth and energy metabolism, by stimulating GH secretion, appetite, and gastric function (Kaiya et al. 2006, 2008; Kang et al. 2011a, 2011b).
Preproghrelin has been identified from several fish species, including goldfish (Unniappan et al. 2002), Japanese eel (Kaiya et al. 2003a), Mozambique tilapia (Kaiya et al. 2003b), rainbow trout (Kaiya et al. 2003c), Nile tilapia (Parhar et al. 2003), channel catfish (Kaiya et al. 2005), sea bream (Yeung et al. 2006), common carp (Kono et al. 2008), zebrafish (Amole and Unniappan 2009), Atlantic cod (Xu and Volkoff 2009), Arctic charr (Frøiland et al. 2010), Pacific bluefin tuna (Suda et al. 2012), crucian carp (Zhou et al. 2012), grass carp (Feng et al. 2013), and David’s schizothoracin (Cai et al. 2014). Gene structure and messenger RNA (mRNA) quantification during fasting and re-feeding provided evidence for preproghrelin’s stimulatory role in food intake, and central and peripheral injections of preproghrelin also increased food intake in goldfish (Unniappan et al. 2002, 2004; Miura et al. 2006; Matsuda et al. 2006). Similarly, after a chronic treatment with native preproghrelin, the food intake and body weight were increased in Mozambique tilapia (Riley et al. 2005). But the aforementioned reports revealed that the function mechanisms of preproghrelin are species-specific, suggesting the necessity of further investigations on the physiological roles of preproghrelin in various fish species (Kaiya et al. 2008).
An understanding of the interactions between environmental factors and the mechanisms of appetite control is fundamental to the development of practical approaches to optimize feed intake, which will usher in a new era of research in redefining the limits of productivity (Matteri 2001). Apart from nutrient availability, temperature and photoperiod are two other important environmental factors that may affect feeding and appetite in fish. However, their effects vary among fish species.
The Chinese perch, Siniperca chuatsi (Basilewsky), has unique food preference (Liang et al. 2001; Liang 2008). In the wild, the fry, from the initiation of feeding, feed solely on live fry of other fish species (Chiang 1959). For many years, to reduce the high production costs of carnivorous fish by domesticating them to feed on artificial diet has been a challenge (Kubitza and Lovshin 1999), and gaining deep insight into the regulation of food intake in carnivorous fish would have great significance in solving this problem. The present study was designed to improve our understanding of the neuroendocrine regulation of food intake in this economically valuable species, by cloning the complementary DNA (cDNA) sequence of preproghrelin, analyzing its structure, tissue distribution, and changes in mRNA expression in various tissues of animals exposed to different short-term fasting, temperatures, and photoperiods. Our results will provide new insights into the physiological roles of preproghrelin in the regulation of the growth and food intake of Chinese perch.
Materials and methods
Animals and samples
The Chinese perch (120 ± 15 g body weight) were obtained from Jiangxia National Fine Breed of Chinese Perch Farm (Jiangxia, Hubei, China) and were acclimated to natural photoperiod (11 h of light and 13 h of dark) and temperature for 2 weeks with a circulating freshwater system before the experiments. Fourteen groups of fish (7 fasted and 7 control groups) were used to evaluate the effect of short-term fasting on preproghrelin mRNA expression in Chinese perch. The fish were maintained separately in 42 plastic aquariums (100 × 50 × 50 cm3) (3 aquariums per group and 8 fish per aquarium). The fish in the control groups were fed to apparent satiation with live mud fish (Misgurnus anguillicaudatus Cantor) once daily at 9:00 a.m., and three fish per group were randomly sampled at 0, 1, 3, 6, 12, 24, and 48 h post-feeding. The fish in fasted groups were not fed at 9:00 a.m. and then sampled at the above indicated time points. The sampled fish were anesthetized in 0.02% tricaine-methanesulfonate (MS-222); the stomach and brain tissues were collected and stored at −80 °C until RNA isolation.
After a 2-week temporary rearing, all fish were randomly divided into four temperature groups (8, 18, 26, 32 °C, 3 aquariums per group and 8 fish per aquarium) and three photoperiod groups (continuous light (CL), continuous dark (CD), and normal light (NL) (11 h of light and 13 h of dark), 3 aquariums per group and 8 fish per aquarium), and then all the fish were fed to satiation with live mud fish once daily at 9:00 a.m. for 2 weeks. Three fish were randomly sampled from each group from the respective aquariums at 9:00 a.m. (fish in both the control group and the fasted group were fasted for 1 day before sampled, which has been used in many similar experiments), and then anesthetized in 0.02% MS-222 before tissue collection. The stomach and brain collected were immediately frozen in liquid nitrogen and stored at −80 °C until total RNA extraction. Other tissues including the cerebellum, diencephalon, telencephalon, pituitary, eye, gill, heart, pyloric caecum, liver, intestinal tract, head kidney, body kidney, gall bladder, spleen, and muscle were collected at natural temperature (18 °C) for detection of the tissue distribution of preproghrelin.
Cloning of preproghrelin in Chinese perch and tissue distribution analysis
Total RNA was extracted using Trizol® Reagent (TaKaRa, Dalian, China) and was treated with RNase-Free DNase I Water (provided in the kit) according to the manufacturer’s instructions. The concentrations and integrity of the RNA were determined by a photometer (Bio-Rad, Hercules, CA, USA) fixed at 260 and 280 nm wavelengths and RNA electrophoresis, followed by storing the total RNA at −80 °C until the next step.
In order to clone Chinese perch preproghrelin open reading frame (ORF), primers (Table 1) were designed based on other fish preproghrelin sequences deposited in the NCBI GenBank (http://www.ncbi.nlm.nih.gov/genbank). PCR reaction was performed in total volume of 25 μL reaction system containing 12.5 μL dNTP Mix (Invitrogen, Carlsbad, CA, USA), 1.25 μL each of sense primer and antisense primers (10 μM), 2.5 μL cDNA, and 7.5 μL ddH2O, under following parameters: pre-denaturation at 94 °C for 4 min, − 30 cycles of 94 °C for 30 s, 57 °C for 30 s, 72 °C for 30 s, and a final extension at 72 °C for 10 min. The PCR products were purified from agarose gel using Universal DNA Purification Kit (Tiangen, Beijing, China), and then cloned into pMD®19-T plasmid vector (TaKaRa,). The inserts were sequenced by automated sequence analysis (TaKaRa).
Structural analysis
Multiple sequence alignments were generated using the Clustal X 2.1. The cleavage site of the signal peptide was estimated using Signal P Ver. 4.0 program (http://www.cbs.dtu.dk/services/ SignalP/). A phylogenetic tree was constructed based on the amino acid sequences by the neighbor-joining method of the Clustal W (http://www.ddbj.nig.ac.jp/search/clustalw-e.html) and MEGA 6.0 program (http://www.megasoftware.net/index.html).
Real-time quantitative PCR
After the sequence was confirmed, the tissue distribution of preproghrelin mRNA was studied in the brain, eye, gill, heart, stomach, pyloric caecum, liver, intestinal, head kidney, body kidney, gall bladder, spleen, and muscle. The preproghrelin mRNA expression after 0, 1, 3, 6, 12, 24, and 48 h of fasting, as well as post-feeding, was studied in the pituitary and stomach. The preproghrelin mRNA expression at 8, 18, 26, and 32 °C, and at different conditions of light, was studied in the brain and stomach
Real-time PCR was carried out on the CFX Connect Real-Time System (Bio-Rad) using SYBR Green (TaKaRa). The primers used are listed in Table 2. All real-time PCR reactions were performed in triplicate. Each PCR mixture (25 μL) contained 12.5 μL of 2 × SYBRR Premix Ex Tap™ (TaKaRa), 0.5 μL of each primer, 2.5 μL of cDNA, and 9.5 μL of RNase-Free H2O. The PCR amplification was performed at 95 °C for 30 s, followed by 45 cycles of 95 °C for 5 s, and 60 °C for 30 s.
Statistical analysis
The β-actin gene was used as a housekeeping gene in this study. The 2–ΔΔCt method was used to determine the relative mRNA abundance for the surveyed samples (Livak and Schmittgen 2001). Treatments that do not share a common letter are significantly different from each other as determined by one-way ANOVA (P < 0.05). In fasting study, fish groups with an asterisk above show significant differences between the control and the experiment group.
Results
Molecular cloning of Chinese perch preproghrelin
From the RACE PCR, the full-length preproghrelin cDNA sequence was obtained. The preproghrelin (GenBank Accession No. KR491948 ) nucleotide sequence of Chinese perch was 434 bp long, containing a 321-bp ORF and a 113-bp 3′-untranslated region (3′-UTR). The deduced preproghrelin peptide was composed of 107 amino acid residues, with an N-terminal 26 amino acid signal peptide, a 20 amino acid mature peptide (GSSFLSPSQKPQNKGKPFRV), a potential amidation-proteolytic site (Gly-Arg), and a 61 amino acid C-terminus peptide of preproghrelin (Fig. 1).
Tissue distribution of preproghrelin mRNA in Chinese perch
Real-time quantitative PCR (RT-qPCR) was performed to analyze preproghrelin mRNA expression in central nervous and peripheral tissues (Fig. 2). Results showed that expression of preproghrelin mRNA was detected in all the tissues tested, with the highest levels observed in the stomach, followed by the pituitary and liver, moderate in the cerebellum, diencephalon, telencephalon, pyloric caecum, intestine, and spleen, and the lowest in the eye, gill, heart, head kidney, body kidney, gall bladder, and muscle.
Expression of preproghrelin in response to fasting
Analysis of preproghrelin mRNA expression in the stomach after different periods of fasting showed that, after gastric emptying (3–6 h), short-term fasting (6–12 h) increases preproghrelin expression when compared to control. This increase in expression was observed until 24 h of fasting; then, preproghrelin levels returned to basal. Before 3 h, incompletely digested prey fish were found in the stomach and preproghrelin expression was lower than basal level. In pituitary, fasting decreased preproghrelin expression at 1, 3, 12, and 48 h but did not exert any change at 6 and 24 h (Fig. 3).
Expression of preproghrelin in fish reared at different temperatures
As shown in Fig. 4, preproghrelin mRNA was expressed at the highest level in the brain and the stomach at 26 and 32 °C, respectively. With the temperature increasing from 8 to 32 °C, the expression level increased all the time in the stomach, but it increased until 26 °C and decreased at 32 °C in the brain.
Expression of preproghrelin at different photoperiods
The expression levels of preproghrelin mRNA in the stomach showed small but statistically significant differences at the different photoperiod tested. The preproghrelin mRNA levels under both CD and CL conditions were significantly lower than those under the NL condition (Fig. 5). Additionally, preproghrelin mRNA levels under CD and CL conditions did not have statistically significant differences in the brain, both of which were significantly lower than those under the NL condition (Fig. 5).
Discussion
In the present study, we obtained the full-length preproghrelin cDNA and predicted mature peptide in Chinese perch. The putative mature peptide of Chinese perch is composed of GSSFLSPSQKPQNKGKPFRV, with the first five amino acids (GSSFL) considered the “active core” (Bednarek et al. 2000). This sequence is the same as that of rainbow trout (Kaiya et al. 2003a), Japanese eel (Kaiya et al. 2003b), Mozambique tilapia (Kaiya et al. 2003c), Nile tilapia (Parhar et al. 2003), channel catfish (Kaiya et al. 2005), sea bream (Yeung et al. 2006), Pacific bluefin tuna (Suda et al. 2012), sea bass (Terova et al. 2008), Atlantic salmon (Murashita et al. 2009), orange-spotted grouper (Chen et al. 2008), and mammals (rat and human) (Kojima et al. 1999), but different from the active core (GTSFL) in goldfish (Unniappan et al. 2002), zebrafish (Amole and Unniappan 2009), and grass carp (Feng et al. 2013) (Supple. File 1). Notably, in the N-terminal portion of the mature preproghrelin peptide, the first seven amino acids are highly conserved, including a serine3 residue, which is the site of acylation, an essential modification for receptor binding and biological activity (Kojima et al. 1999). The mature preproghrelin peptides in vertebrates vary in their length—28 amino acids for rats and humans (Kojima et al. 1999), but 20 amino acids for Chinese perch, bluefin tuna (Suda et al. 2012), sea bream (Yeung et al. 2006), sea bass (Terova et al. 2008), and Nile tilapia (Parhar et al. 2003).
As in mammals, preproghrelin is primarily produced in the stomach and intestine (stomach-less) of fish, but also detected in the kidney, hypothalamus, heart, brain, and gills (Unniappan et al. 2002; Parhar et al. 2003; Kono et al. 2008). In our study, preproghrelin mRNA was primarily expressed in the stomach of Chinese perch, consistent with the finding in mammals (Ariyasu et al. 2001). In Chinese perch, preproghrelin mRNA expression level in the brain and liver was only a little lower than that in the stomach, which was similar to the results in goldfish (Unniappan et al. 2004), rainbow trout (Kaiya et al. 2003a), Japanese eel (Kaiya et al. 2003b), Mozambique tilapia (Peddu et al. 2009), hammerhead shark (Kawakoshi et al. 2007), and Atlantic cod (Xu and Volkoff 2009), indicating the important roles of stomach, brain and liver in preproghrelin secretion. Furthermore, the expression of preproghrelin mRNA was detected in all the tissues studied, similar to previous studies on preproghrelin mRNA in human tissues (Gnanapavan et al. 2002) and the tissues of several fish species (Kaiya et al. 2008).
The effect of fasting on the expression level of preproghrelin mRNA was studied in zebrafish, and in both the gut and brain the expression level increased significantly by fasting, but declined sharply after re-feeding (Amole and Unniappan 2009). In Chinese perch, the potential role of preproghrelin in the regulation of appetite and food intake was further supported by fasting-induced up-regulation of preproghrelin mRNA expression in the stomach from 6 to 12 h fasting. At 3 h fasting, incompletely digested prey fish were found in the stomach and preproghrelin expression was low. After 3 h fasting, preproghrelin in the stomach increased significantly. This can also be seen in goldfish (Unniappan et al. 2004) and sea bass (Terova et al. 2008), but no change is observed in rainbow trout (Jönsson et al. 2007). No effect on preproghrelin mRNA by fasting or re-feeding was found in Nile tilapia and Atlantic cod (Parhar et al. 2003; Xu & Volkoff 2009). These results suggest that the preproghrelin physiology varies in fish. In the present study, the preproghrelin mRNA expression in the stomach of Chinese perch was more sensitive (relative expression level from 0.3 to 3.5) to fasting than that in the pituitary/brain (relative expression level from 0.2 to 1.7). During the entire process of fasting, preproghrelin expression in the pituitary presented state fluctuation of self-adjustment with up and downregulation.
To further improve the growth rate of fish, it is necessary to increase the food intake, which is closely related with two important environmental factors: temperature and photoperiod (Volkoff et al. 2009). However, the individual effects of the two factors are very difficult to determine because fish is subjected to seasonal cycles and both parameters vary under natural conditions.
In this study, the preproghrelin mRNA expression was higher in both the stomach and the brain at 26 °C than at a lower temperature, but lower in the brain at 32 °C than at 26 °C, suggesting that the higher the temperature is, the more the preproghrelin expression is in the stomach and the stomach has a higher optimal temperature than the brain for preproghrelin expression. In some fish species, food consumption and growth rates tend to increase with rising temperature (Bendiksen et al. 2002; Sunuma et al. 2007). The food intake of grass carp is also regulated by water temperature (Wen et al. 1998). In the burbot, fasting decreases plasma preproghrelin-immunoreactive peptide levels at 2 °C but not at 10 °C (Nieminen et al. 2003). Picha et al. (2009) reported that blood preproghrelin of hybrid striped bass increases significantly by fasting at 14 and 24 °C. Xu and Volkoff (2009) found that during fasting, preproghrelin mRNA expression remained unchanged during catabolism in Atlantic cod, but plasma preproghrelin-immunoreactive peptide levels decrease in linear relation with the temperature at 20 °C. Two recent studies on Atlantic salmon generated conflicting results. In one study, when the Atlantic salmon were kept at different temperatures for 3 months, their growth and food intake are decreased at 19 °C compared to fish at 14 °C (Hevrøy et al. 2012) while in the other study, the Atlantic salmon showed no significant difference in plasma preproghrelin levels at three different temperatures (8, 12, and 18 °C) (Kullgren et al. 2013). In summary, high temperature increases appetite to some extent in most cases, but some cold water fish adapt to low temperature and have stronger appetite in a low temperature.
Additionally, both continuous dark and continuous light reduced preproghrelin mRNA expression compared to the normal light (Fig. 5). Previous studies showed that feeding activity is affected by photoperiod and light regimens in a number of fish species including European sea bass (Sanchez-Vazquez et al. 1998), yellowtail (Kohbara et al. 2000), and barfin flounder (Sunuma et al. 2007). However, Atlantic cod showed no obvious differences in neither food intake nor preproghrelin mRNA expression under different photoperiods (24 h light, 24 h dark, 16 h light: 8 h dark) (Xu and Volkoff 2009). Above studies indicated that photoperiod may affect food intake, but this effect is species-specific and may have relationship with surroundings.
The endocrine mechanism for the regulation of feeding by environmental factors (fasting, temperature, and photoperiod) is interactive. Future studies should focus on the interaction of these three key factors as well as tissue-specific effects on preproghrelin mRNA expression to further understand the physiological roles of preproghrelin in Chinese perch.
Conclusion
In this study, we characterized the structure of preproghrelin cDNA, the deduced mature peptide and tissue expression of preproghrelin mRNA in Chinese perch. The widespread distribution of preproghrelin mRNA in tissues implicated in the regulation of metabolism (such as the stomach, brain, liver, and spleen) suggested that preproghrelin might play an important role in energy balance in Chinese perch. Interactions between environmental factors and the mechanisms of appetite control are fundamental to the development of practical approaches to optimize feed intake. Fasting-induced increase of preproghrelin mRNA expression in the stomach suggests an orexigenic role of preproghrelin in Chinese perch. Higher temperature increased the level of preproghrelin mRNA expression in the stomach, which had a higher optimal temperature (32 °C) than the brain (26 °C). Additionally, the normal light is an appropriate photoperiod for Chinese perch growth. These findings suggest that short-term fasting of 6 h after gastric emptying, 26 °C, and normal light would be appropriate for culturing Chinese perch. The overall results from this study provide some insights into preproghrelin mRNA expression of Chinese perch in response to fasting, temperature, and photoperiod as well as useful information for culturing this valuable fish species.
References
Amole N, Unniappan S (2009) Fasting induces preproghrelin mRNA expression in the brain and gut of zebrafish, Danio rerio. Gen Comp Endocrinol 161:133–137
Ariyasu H, Takaya K, Tagami T, Ogawa Y, Hosoda K, Akamizu T, Suda M, Koh T, Natsui K, Toyooka S, Shirakami G, Usui T, Shimatsu A, Doi K, Hosoda H, Kojima M, Kanqawa K, Nakao K (2001) Stomach is a major source of circulating ghrelin, and feeding state determines plasma ghrelin-like immunoreactivity levels in humans. J Clin Endocrinol Metab 86:4753–4758
Bednarek MA, Feighner SD, Pong SS, McKee KK, Hreniuk DL, Silva MV, Warren VA, Howard AD, Van Der Ploeq LH, Heck JV (2000) Structure-function studies on the new growth hormone-releasing peptide, ghrelin: minimal sequence of ghrelin necessary for activation of growth hormone secretagogue receptor 1a. J Med Chem 43:4370–4376
Bendiksen E, Jobling M, Arnesen A (2002) Feed intake of Atlantic salmon parr Salmo salar L. in relation to temperature and feed composition. Aquac Res 33:525–532
Bernier NJ, Peter RE (2001) The hypothalamic–pituitary–interrenal axis and the control of food intake in teleost fish. Comp Biochem Phys B 129(2):639–644
Cai L, Liu G, Taupier R, Fang M, Johnson D, Tu Z, Huang Y (2014) Effect of temperature on swimming performance of juvenile Schizothorax prenanti. Fish Physiolo Biochem 40(2):491–498
Chen T, Tang Z, Yan A, Li W, Lin H (2008) Molecular cloning and mRNA expression analysis of two GH secretagogue receptor transcripts in orange-spotted grouper (Epinephelus coioides). J Endocrinol 199(2):253–265
Chiang IK (1959) On the biology of mandarin fish, Siniperca chuatsi of Liang-Tze Lake. Acta Hydrobiol Sin 3:375–385
Feng KE, Zhang GR, Wei KJ, Xiong BX (2013) Molecular cloning, tissue distribution, and ontogenetic expression of ghrelin and regulation of expression by fasting and refeeding in the grass carp (Ctenopharyngodon idellus). J Exp Zool A 319:202–212
Frøiland E, Murashita K, Jørgensen EH, Kurokawa T (2010) Leptin and ghrelin in anadromous Arctic charr: cloning and change in expressions during a seasonal feeding cycle. Gen Comp Endocr 165(1):136–143
Gnanapavan S, Kola B, Bustin SA, Morris DG, McGee P, Fairclough P, Bhattacharya S, Carpenter R, Grossman AB, Korbonits M (2002) The tissue distribution of the mRNA of ghrelin and subtypes of its receptor, GHS-R, in humans. J Clin Endocrinol Metab 87:2988–2988
Hevrøy EM, Waagbø R, Torstensen BE, Takle H, Stubhaug I, Jørgensen SM, Torgersen T, Tvenning L, Susort S, Breck O, Hansen T (2012) Ghrelin is involved in voluntary anorexia in Atlantic salmon raised at elevated sea temperatures. Gen Comp Endocrinol 175:118–134
Jönsson E, Forsman A, Einarsdottir IE, Kaiya H, Ruohonen K, Björnsson BT (2007) Plasma ghrelin levels in rainbow trout in response to fasting, feeding and food composition, and effects of ghrelin on voluntary food intake. Comp Biochem Phys A 147:1116–1124
Kaiya H, Kojima M, Hosoda H, Moriyama S, Takahashi A, Kawauchi H, Kangawa K (2003a) Peptide purification, complementary deoxyribonucleic acid (DNA) and genomic DNA cloning, and functional characterization of ghrelin in rainbow trout. Endocrinology 144:5215–5226
Kaiya H, Kojima M, Hosoda H, Riley LG, Hirano T, Grau EG, Kangawa K (2003b) Amidated fish ghrelin: purification, cDNA cloning in the Japanese eel and its biological activity. J Endocrinol 176:415–423
Kaiya H, Kojima M, Hosoda H, Riley LG, Hirano T, Grau EG, Kangawa K (2003c) Identification of tilapia ghrelin and its effects on growth hormone and prolactin release in the tilapia, Oreochromis mossambicus. Comp Biochem Phys B 135:421–429
Kaiya H, Small BC, Bilodeau AL, Shepherd BS, Kojima M, Hosoda H, Kangawa K (2005) Purification, cDNA cloning, and characterization of ghrelin in channel catfish, Ictalurus punctatus. Gen Comp Endocr 143:201–210
Kaiya H, Tsukada T, Yuge S, Mondo H, Kangawa K, Takei Y (2006) Identification of eel ghrelin in plasma and stomach by radioimmunoassay and histochemistry. Gen Comp Endocrinol 148:375–382
Kaiya H, Miyazato M, Kangawa K, Peter RE, Unniappan S (2008) Ghrelin: a multifunctional hormone in non-mammalian vertebrates. Comp Biochem Phys A 149:109–128
Kang KS, Yahashi S, Matsuda K (2011a) Central and peripheral effects of ghrelin on energy balance, food intake and lipid metabolism in teleost fish. Peptides 32:2242–2247
Kang KS, Yahashi S, Matsuda K (2011b) The effects of ghrelin on energy balance and psychomotor activity in a goldfish model: an overview. Int J Peptides 2011:1–9
Kawakoshi A, Kaiya H, Riley LG, Hirano T, Grau EG, Miyazato M, Kangawa K (2007) Identification of a ghrelin-like peptide in two species of shark, Sphyrna lewini and Carcharhinus melanopterus. Gen Comp Endocr 151(3):259–268
Kohbara J, Hidaka I, Kuriyama I, Yamashita M, Ichikawa M, Furukawa K, Aida K, Sanchez-Vazquez FJ, Tabata M (2000) Nocturnal/diurnal demand-feeding pattern of yellowtail Seriola quinqueradiata under different keeping conditions. Fish Sci 66:955–962
Kojima M, Hosoda H, Date Y, Nakazato M, Matsuo H, Kangawa K (1999) Ghrelin is a growth-hormone-releasing acylated peptide from stomach. Nature 402:656–660
Kono T, Kitao Y, Sonoda K, Nomoto R, Mekata T, Sakai M (2008) Identification and expression analysis of ghrelin gene in common carp Cyprinus carpio. Fish Sci 74:603–612
Kubitza F, Lovshin LL (1999) Formulated diets, feeding strategies, and cannibalism control during intensive culture of juvenile carnivorous fishes. Rev Fish Sci 7:1–22
Kullgren A, Jutfelt F, Fontanillas R, Sundell K, Samuelsson L, Wiklander K, Kling P, Koppe W, Joakim Larsson DG, Björnsson TB, Jönsson E (2013) The impact of temperature on the metabolome and endocrine metabolic signals in Atlantic salmon (Salmo salar). Comp Biochem Phys A 164:44–53
Liang XF, Oku H, Ogata HY, Liu J, He X (2001) Weaning Chinese perch Siniperca chuatsi (Basilewsky) onto artificial diets based upon its specific sensory modality in feeding. Aquac Res 36:1588–1594
Liang XF, Lin XT, Li SQ, Liu JK (2008) Impact of environmental and innate factors on the food habit of Chinese perch Siniperca chuatsi (Basilewsky) (Percichthyidae). Aquac Res 39:150–157
Livak KJ, Schmittgen TD (2001) Analysis of relative gene expression data using real-time quantitative PCR and the 2−ΔΔCT method. Methods 25:402–408
Matsuda K, Miura T, Kaiya H, Maruyama K, Shimakura SI, Uchiyama M, Shioda S (2006) Regulation of food intake by acyl and des-acyl ghrelins in the goldfish. Peptides 27(9):2321–2325
Matteri RL (2001) Overview of central targets for appetite regulation. J Anim Sci 79(E-Suppl):E148–E158
Miura T, Maruyama K, Shimakura SI, Kaiya H, Uchiyama M, Kangawa K, Shioda S, Matsuda K (2006) Neuropeptide Y mediates ghrelin-induced feeding in the goldfish, Carassius auratus. Neurosci Lett 407:279–283
Murashita K, Kurokawa T, Nilsen TO, Rønnestad I (2009) Ghrelin, cholecystokinin, and peptide YY in Atlantic salmon (Salmo salar): molecular cloning and tissue expression. Gen Comp Endocr 160(3):223–235
Nakazato M, Murakami N, Date Y, Kojima M, Matsuo H, Kangawa K, Matsukura S (2001) A role for ghrelin in the central regulation of feeding. Nature 409:194–198
Nieminen P, Mustonen AM, Hyvärinen H (2003) Fasting reduces plasma leptin- and ghrelin-immunoreactive peptide concentrations of the burbot (Lota lota) at 2 °C but not at 10 °C. Zool Sci 20:1109–1115
Parhar IS, Sato H, Sakuma Y (2003) Ghrelin gene in cichlid fish is modulated by sex and development. Biochem Biophys Res Commun 305:169–175
Peddu SC, Breves JP, Kaiya H, Grau EG, Riley LG (2009) Pre-and postprandial effects on ghrelin signaling in the brain and on the GH/IGF-I axis in the Mozambique tilapia (Oreochromis mossambicus). Gen Comp Endocr 161(3):412–418
Pfaff, D (1969) Sex differences in food intake changes following pituitary growth hormone or prolactin injections. In Proceedings of the Annual Convention of the American Psychological Association. American Psychological Association.
Picha ME, Strom CN, Riley LG, Walker AA, Won ET, Johnstone WM, Borski RJ (2009) Plasma ghrelin and growth hormone regulation in response to metabolic state in hybrid striped bass: effects of feeding, ghrelin and insulin-like growth factor-I on in vivo and in vitro GH secretion. Gen Comp Endocr 161:365–372
Riley LG, Fox BK, Kaiya H, Hirano T, Grau EG (2005) Long-term treatment of ghrelin stimulates feeding, fat deposition, and alters the GH/IGF-I axis in the tilapia, Oreochromis mossambicus. Gen Comp Endocr 142:234–240
Sanchez-Vazquez FJ, Azzaydi M, Martinez FJ, Zamora S, Madrid JA (1998) Annual rhythms of demand-feeding activity in sea bass: evidence of a seasonal phase inversion of the diel feeding pattern. Chronobiol Int 15:607–622
Suda A, Kaiya H, Nikaido H, Shiozawa S, Mishiro K, Ando H (2012) Identification and gene expression analyses of ghrelin in the stomach of Pacific bluefin tuna (Thunnus orientalis). Gen Comp Endocrinol 178:89–97
Sunuma T, Amano M, Yamanome T, Furukawa K, Yamamori K (2007) Self-feeding activity of a pleuronectiform fish, the barfin flounder. Aquaculture 270:566–569
Terova G, Rimoldi S, Bernardini G, Gornati R, Saroglia M (2008) Sea bass ghrelin: molecular cloning and mRNA quantification during fasting and refeeding. Gen Comp Endocrinol 155:341–351
Unniappan S, Lin X, Cervini L, Rivier J, Kaiya H, Kangawa K, Peter RE (2002) Goldfish ghrelin: molecular characterization of the complementary deoxyribonucleic acid, partial gene structure and evidence for its stimulatory role in food intake. Endocrinology 143:4143–4146
Unniappan S, Canosa LF, Peter RE (2004) Orexigenic actions of ghrelin in goldfish: feeding-induced changes in brain and gut mRNA expression and serum levels, and responses to central and peripheral injections. Neuroendocrinology 79:100–108
Volkoff H, Xu M, MacDonald E, Hoskins L (2009) Aspects of the hormonal regulation of appetite in fish with emphasis on goldfish, Atlantic cod and winter flounder: notes on actions and responses to nutritional, environmental and reproductive changes. Comp Biochem Physiol A 153:8–12
Wang G, Lee HM, Englander E, Greeley GH (2002) Ghrelin not just another stomach hormone. Regul Peptides 105(2):75–81
Wen LY, Tan YJ, Wang W (1998) Effects of water temperature on feeding, growth and mortality of grass carp fingerlings. J Fish China 22:371–374
Wren AM, Small CJ, Ward HL, Murphy KG, Dakin CL, Taheri S, Bloom SR (2000) The novel hypothalamic peptide ghrelin stimulates food intake and growth hormone secretion. Endocrinology 141:4325–4328
Xu M, Volkoff H (2009) Molecular characterization of ghrelin and gastrin-releasing peptide in Atlantic cod (Gadus morhua): cloning, localization, developmental profile and role in food intake regulation. Gen Comp Endocrinol 160:250–258
Yeung CM, Chan CB, Woo NY, Cheng CH (2006) Sea bream ghrelin: cDNA cloning, genomic organization and promoter studies. J Endocrinol 189:365–379
Zhou C, Zhang X, Liu T, Wei R, Yuan D, Li Z (2012) Cloning and prokaryotic expression of ghrelin gene in crucian carp (Carassius auratus). Afr J Microbiol Res 6(24):5222–5228
Acknowledgements
This work was financially supported by the National Natural Science Foundation of China (31272641), the Key Projects in the National Science & Technology Pillar Program (2012BAD25B04), and the Fundamental Research Funds for the Central Universities (2662015PY041 and 2015BQ040).
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Song, Y., Zhao, C., Liang, Xf. et al. Effects of fasting, temperature, and photoperiod on preproghrelin mRNA expression in Chinese perch. Fish Physiol Biochem 43, 803–812 (2017). https://doi.org/10.1007/s10695-016-0335-y
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DOI: https://doi.org/10.1007/s10695-016-0335-y