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1 February 2003 Steroidogenic Acute Regulatory Protein in Eels: cDNA Cloning and Effects of ACTH and Seawater Transfer on Its mRNA Expression
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Abstract

Steroidogenic acute regulatory protein (StAR) is a key molecule for steroid production by translocating cholesterol from the outer to inner mitochondrial membrane. Two cDNAs of different length encoding StAR was cloned from the head kidney of the eel (Anguilla japonica). In the 3′-untranslated region (UTR) of the longer cDNA, two putative polyadenylation signals were found. The shorter one differed from the longer one solely by the lack of middle of 3′-UTR including the first polyadenylation signal. Reverse transcription-polymerase chain reaction (RT-PCR) that differentiates the two mRNAs showed that the ratio of the two was highly variable among individuals, and no preferential expression was detected between freshwater and seawater eels. The predicted protein consists of 285 amino acid residues with 64–83% identity to other StARs thus far obtained. RT-PCR analyses revealed that eel StAR mRNA was expressed abundantly in the head kidney and gonad, and faintly in the brain; but no expression was detected in the gill, heart, liver, intestine, kidney and skeletal muscle. Plasma cortisol concentration increased, but StAR mRNA content in the head kidney did not change, 3 and 24 h after transfer of freshwater eels to seawater, indicating that the transcriptional regulation of StAR may not be involved in cortisol production after seawater transfer. However, ACTH elevated both plasma cortisol and StAR mRNA levels in the head kidney 1.5 and 4.5 h after injection. Thus, the steroidogenic effect of ACTH is mediated by increased StAR production as observed in mammals.

INTRODUCTION

The biosynthesis of steroids begins with the conversion of cholesterol to pregnenolone, which is catalyzed by cyto-chrome P450 side chain cleavage enzyme (P450scc). It is known, in mammals, that the delivery of cholesterol from the outer to the inner mitochondrial membrane, where P450scc resides, is the rate-limiting step in steroidogenesis, and a mediator called steroidogenic acute regulatory protein (StAR) is required for this process (Stocco, 2001). It appears that this protein plays a critical role in the regulation of hormonally induced acute steroid production by stimulating cholesterol transfer through the hydrophobic tunnel structure formed within its molecule (Tsujishita and Hurley, 2000; Stocco, 2001).

The cDNA encoding StAR has been cloned in various mammalian species such as the mouse (Clark et al., 1994), human (Sugawara et al., 1995), rat (Ariyoshi et al., 1998), hamster (Fleury et al., 1998), and horse (Kerban et al., 1999). In these animals, most steroidogenic actions of hormones and other factors are due to the increased StAR expression (Kerban et al., 1999; Stocco 2001). In non-mammalian vertebrates, StAR cDNAs have also been cloned in the chicken (Gallus gallus), Xenopus laevis, zebrafish (Danio rerio) and trout (Salvelinus fontinalis and Oncorhynchus mykiss) (Bauer et al., 2000; Kusakabe et al., 2002). The primary structure of StAR and tissue distribution of its transcripts are basically similar to those in mammals. However, little is known about the functional role of StAR in non-mammalian vertebrates except for the recent data that gonadotropins stimulated StAR expression in the follicle cells of the hen in vitro (Johnson and Bridgham, 2001), and that acute stress increased StAR transcripts in the head kidney of the trout (Kusakabe et al., 2002).

Cortisol is a principal corticosteroid secreted from the interrenal (the adrenocortical homologue) located in the head kidney of teleosts, and plays a pivotal role in adaptation to both freshwater (FW) and seawater (SW) environments (for review, see McCormick 2001). Several hormones such as adrenocorticotropin (ACTH), natriuretic peptides (NPs), angiotensin II (ANG II) and urotensins have been shown to stimulate cortisol secretion in teleost fish (Henderson et al., 1976; Arnold-Reed and Balment, 1994; Li and Takei, 2003), and some of the hormones have been implicated in SW adaptation (Takei, 1993). However, little is known about the mechanisms by which these hormones stimulate cortisol production in fish. One possibility is that these hormones activate the steroidogenic enzymes involved in cortisol synthesis (Miller, 1988). Recent evidence in mammals raises the possible involvement of StAR in the hormonally induced cortisol production in fish. For examining it, the cDNA encoding StAR was cloned from the head kidney of a euryhaline teleost, the eel (Anguilla japonica) in the present study. The tissue distribution of StAR mRNA was examined by RT-PCR. In addition, changes in plasma cortisol concentrations were examined together with StAR mRNA expression in the head kidney after ACTH injection or transfer of eels from FW to SW, to assess whether StAR is involved in the cortisol production caused by hormonal and environmental stimuli.

MATERIALS AND METHODS

Animals and tissues collection

Cultured immature FW eels (Anguilla japonica) were purchased from a local dealer. The gonads were immature, and thus the sex was indistinguishable by naked eye. Eels were maintained under natural photoperiod in FW or SW tanks for more than one or two weeks, respectively, before experimental use. Water in the tank was continuously circulated, aerated, and regulated at 18°C. After anesthetization of eels with 0.1% (w/v) tricaine methanesulfonate (MS-222) (Sigma, St. Louis, USA), the tissues (see Tissue distribution) were surgically isolated and immediately frozen in liquid nitrogen, and were then stored at −80°C until RNA extraction.

RNA extraction

Total RNA was extracted from various tissues using ISOGEN (Nippon Gene, Toyama, Japan). For cDNA cloning, poly (A)+-RNA was subsequently isolated from the total RNA extracted from the head kidney of a FW eel using Oligotex-dT30 (Japan Synthetic Rubber, Tokyo, Japan).

Cloning of eel StAR cDNA

The double-stranded cDNA pool was prepared from 0.5 μg poly (A)+-RNA using SMART cDNA Library Construction Kit (Clontech Laboratories, Palo Alto, CA) as described previously (Inoue et al., 2003). Degenerate primer S1 [5′-GCAACHTTCAAAYTGTGYGC-3′] and A1 [5′-TTCCASTCVCCCATYTGYTCCAT-3′] (Fig. 1), which were designed based on the StAR cDNA sequences of zebrafish (accession no.  AF220435), trout ( AF232215,  AB047032), Xenopus laevisAF220437) and chicken ( AF220436), were used to amplify a partial cDNA fragment. Thirty cycles of amplification (denaturation at 94°C for 30 s, annealing at 61°C for 60 s and extension at 72°C for 90 s) were performed using Ex Taq DNA polymerase (Takara Shuzo, Kyoto, Japan). The amplified cDNA fragments were electrophoresed in 1.2% agarose gels containing ethidium bromide (EB), isolated from the gel using Geneclean Kit (Bio101, Vista, CA), subcloned into pT7Blue T-vector (Novagen, Madison, WI) and sequenced in a 310 DNA sequencer (PE Biosystems, Foster City, CA).

5′- and 3′-rapid amplification of cDNA end (RACE) were subsequently performed using the PCR protocol as above. The primers used were gene-specific primers (A2, 5′-CTCAGCACCTTGT CTCCATTG-3′; S2, 5′-CAACCTGTATGGGGAGCTGGT-3′) (Fig. 1) and adaptor primers (5′ PCR primer and CDS III/3′ primer from Clontech), respectively. The PCR products were isolated, sub-cloned and sequenced as above. The full-length of eel StAR cDNA was constructed by aligning the three overlapping cDNA fragments: i.e., the fragment amplified with primers S1 and A1, and the 5′ and 3′ RACE products. Finally, the full coding region was amplified using gene-specific primers S3 (5′-GTATTATCTCGACTGGCTTCG-3′) and A3 (5′-ATCAGCAAGCCTGTGCTGC-3′), which were designed, respectively, from the 5′-UTR end and termination codon region (Fig. 1), to confirm the sequence.

Tissue distribution of mRNA

The tissue distribution of StAR mRNA was evaluated by RTPCR. Examined tissues included the head kidney, kidney, brain, heart, liver, skeletal muscle, immature gonad, intestine and gill from five FW eels (184.3±11.8 g BW) and two SW eels (173.5±10.4 g BW). Total RNA (2 μg) from each tissue was reverse transcribed (RT) with Superscript First Strand Synthesis System (Invitrogen, Carlsbad, CA). Negative control was also run, where the reverse transcriptase was removed from the reaction mixture when performed RT, to confirm the absence of genomic DNA contamination. PCR was carried out for 32 cycles at 94°C for 30 s, 60°C for 30 s and 72°C for 45 s. The expression of eel glyceraldehyde-3-phosphate dehydrogenase (GAPDH) was used as internal control as described previously (Takei et al., 2001). The PCR products were electrophoresed in 1–1.2% agarose gels containing EB, and observed under FAS-III Electronic U.V. Transilluminator (TOYOBO, Osaka, Japan).

Effects of ACTH and SW transfer on plasma cortisol and StAR mRNA levels

Effects of ACTH injection

After FW eels (186.5+13.4 g, n=20) were anesthetized in 0.1% MS-222, a polyethylene tube (SP 10, o.d.=0.61 mm, Natsume Seisakusho Co. Ltd, Tokyo) was surgically inserted into the ventral aorta for blood sampling and ACTH injection. After surgery, eels were held in individual plastic troughs, through which aerated and filtered FW was continuously circulated at 18°C. The troughs were covered with a black vinyl sheet to minimize the visual stress during experiments. On the day after surgery, each eel was given a single injection of ACTH (human, 1–24) (Peptide Institute Inc., Osaka) dissolved in 0.9% NaCl solution at 0.2 nmol/kg in a volume of 0.05 ml. Injection of the same volume of vehicle served as control. Eel ACTH (accession no.  AF194969) is only one-amino acid different from human ACTH (P01189) in the N-terminal 18 amino acids, where the biological activity resides (Dewied, 1990). Since the results in mammals showed that the peak increase of StAR mRNA levels usually occurred at 3–6 hr after ACTH treatment, while plasma cortisol increased in a very short time (5–30 min) (Ariyoshi et al., 1998; LeHoux et al., 1998; Le Roy et al., 2000), we chose two time points (1.5 and 4.5 hr after injection), in this study, to collect blood (ca. 30 μl) and head kidney samples to assess whether StAR was involved in the ACTH-induced cortisol production in eels. Besides, blood was also collected at 0.5 hr after ACTH injection to examine whether cortisol was increased as quickly as observed in mammals. The removed blood volume was replaced immediately by a vehicle injection. After centrifugation, plasma was collected and stored at −20°C for subsequent cortisol determination. Head kidneys were collected for RNA extraction from half of the experimental eels at 1.5 and 4.5 hr after ACTH or saline injection, respectively.

Effects of SW transfer

Thirty FW eels (187.6±15.4 g BW) were equally divided into 5 groups: (1) 0-hr controls, (2) 3-hr FW-FW group, (3) 24-hr FW-FW group, (4) 3-hr FW-SW group, and (5) 24-hr FW-SW group. Plasma cortisol increased within 24 hr after SW transfer in American eel (Anguilla rostrata) (Forrest et al., 1973), so we chose two time points (3 and 24 hr) in this study. The FW-FW groups served as matched time controls. Initially, eels were carefully transferred from a 1-ton FW culture tank to individual 55×40×30 cm experimental tanks with FW for acclimation to new environments. On the next day, water in the experimental tank was carefully decreased to 1/5. For 0-hr controls, eels were then anesthetized in 0.1% MS-222 neutralized with NaHCO3; For FW-FW and FW-SW groups, FW and SW was carefully added, respectively, and fish were anesthetized at 3 or 24 hr after the add of water. Water in the tank was continuously aerated, and regulated at 18°C. The time schedule was arranged to anesthetize the fish between 1300–1400 hr, because it has been shown that plasma cortisol concentration is relatively low and stable around the time of the day (Li and Takei, 2003). After anesthesia, plasma and head kidneys were collected for cortisol determination and RNA extraction, respectively.

Measurement of StAR mRNA content in the head kidney

The content of StAR mRNA in the head kidney was determined by RT-PCR using the protocol similar to that for examining tissue distribution. PCR cycles were changed to 24 for StAR (using primer pair S3-A2) and 26 for GAPDH. In pilot experiments using serially diluted templates, we confirmed that the signal intensity of PCR products and the amount of template exhibited linear relationship under these conditions, and the signal of all experimental samples were within the linear range (data not shown). Each PCR product (10 μl) was electrophoresed in 1.2% EB-stained agarose gels, and the signal was scanned and quantitated using a Fuji FLA-2000 imaging analyzer. The GAPDH signal was also quantified and used to normalize the results of StAR. This process was repeated three times.

Comparison of expression of different StAR transcripts

As will be mentioned below, two transcripts with different length of 3′-UTR have been cloned (Fig. 1). The difference in their expression was examined in the head kidney by RT-PCR. PCR was first conducted using primer pair S3-A3, which amplifies the whole coding region of eel StAR, to confirm the normal expression of StAR in all eels. PCR was then performed using primers S2 and A4 (5′-TATTTGCCGAGCCAG GGTG-3′), of which A4 was located near the poly (A) tail, to distinguish the expression of two transcripts by the length of PCR products. Eels examined in this experiment were 0-hr controls, 3-hr FW-SW and 24-h FW-SW groups of the SW transfer experiment.

Measurement of plasma cortisol and Na±

Plasma cortisol was analysed by enzyme immunoassay (EIA) as described previously (Li and Takei, 2003). In brief, cortisol was extracted from plasma with diethyl ether. In plate wells, 50 μl of cortisol standard (0.04 to 10 ng/ml) or sample were incubated with 50 μl of anti-cortisol serum (1:50000 dilution) and 50 μl of enzyme conjugate (1:1000 dilution) for 1.5 hr at room temperature. After washing, 150 μl of substrate solution was added, incubated for 1 hr at 37°C, and the absorbance was measured at 492 nm in a microplate reader (MTP-300, Corona Electric Co., Ibaragi, Japan). The Na+concentration in plasma of SW-transferred eels was determined in an atomic absorption spectrophotometer (Z5300 Hitachi, Tokyo). Each measurement was performed in duplicate for cortisol and trip-licate for Na+.

Statistics

All data are presented as means ± SEM. Paired t-test was used to determine statistical differences of plasma cortisol concentrations before and after ACTH injection in the same fish. For comparison of plasma cortisol and StAR mRNA levels between ACTHand saline-injected eels, or between FW- and SW-transferred eels, Student's t-test and ANOVA followed by Bonferroni's post-hoc test were applied. Significance was set at p<0.05.

RESULTS

Nucleotide and amino acid sequences of eel StAR

Using a combination of RT-PCR and RACE, two StAR cDNAs differing in the length of 3′-UTR were isolated from the eel head kidney (Fig. 1). The longer cDNA (accession no.  AB095110) consisted of 1451 bp nucleotides (excluding poly (A) tail) containing an 858-bp open reading frame with 66 bp of 5′-UTR and 527 bp of 3′-UTR. In the 3′-UTR, two possible polyadenylation signals were found. The shorter cDNA consisted of 1111 bp, and had the same sequence as the longer one except for the lack of a 340-bp sequence at the central part of the 3′-UTR. The deleted sequence contained the first polyadenylation signal. Both cDNAs encoded an identical peptide with 285 amino acid residues. The percent homologies of eel StAR at the level of nucleotide and amino acid (in parentheses) were 78.2 (82.6) with trout, 73.7 (78.6) with zebrafish, 68.0 (75.2) with Xenopus, 75.0 (76.1) with chicken, and 66.4–70.0 (65.3–67.1) with mammals. The similarity is particularly high in the N-terminus and the functional domains of the C-terminus (Fig. 2).

Fig. 1

Nucleotide and predicted peptide sequences of eel StAR cDNA. Two types of cDNA were isolated from the head kidney. Compared with the longer variant, the shorter one lacks a 340-bp sequence in the 3′-untranslated region (UTR) as indicated by the box. Both 5′- and 3′-UTRs are in lower case; the upper case letters indicate the nucleotides of the coding region. Nucleotide and amino acid numbers are shown on the right. The start (ATG) and termination (TGA) codons are boldfaced. Two putative polyadenylation signals, ‘attaaa’ and ‘aataaa’, are underlined. Primer sequences used for cloning and examining the expression of StAR mRNA are indicated by arrows (see details in Materials and Methods).

i0289-0003-20-2-211-f01.gif

Fig. 2

Alignment of the deduced amino acid sequence of eel StAR with those of other species analyzed by ClustalW multiple alignment. The sequences were obtained from the GenBank database: trout ( AAG39689), zebrafish ( AAG28593), chicken ( AAG28594), rat ( P97826), Human ( P49675). Amino acid numbers are shown on the right. Dashes (-) represent identical amino acid residues and dots (.) represent gaps. The N-terminal 25 residues are indicated by a solid horizontal line. Sites of protein kinase A-mediated phosphorylation of StAR are boxed. The conserved residues important for the steroidogenic function of StAR are indicated by asterisks (*); those putatively directly contributing to the hydrophobic tunnel structure are highlighted by gray boxes.

i0289-0003-20-2-211-f02.gif

Tissue-specific expression of eel StAR mRNA

The expression of StAR mRNA was consistently detected in steroidogenic tissues in both FW and SW eels examined: a high expression was observed in the head kidney and gonad, and a weak expression was encountered in the brain (Fig. 3). However, the expression in other tissues, such as the kidney, heart, intestine, liver, gill, and skeletal muscle, was too low to be detected under the current RTPCR condition.

Fig. 3

Tissue-specific expression of StAR mRNA in eels examined by RT-PCR. The expression of eel glyceraldehyde-3-phosphate dehydrogenase (GAPDH) was used as internal control. Five freshwater and two seawater eels were examined, and the expression patterns were the same. The results for a freshwater eel are presented here.

i0289-0003-20-2-211-f03.gif

Effects of ACTH injection on plasma cortisol and StAR mRNA in head kidney

As shown in Fig. 4, plasma cortisol concentrations increased at 0.5, 1.5 and 4.5 hr after ACTH injection, respectively, compared with the pre-injection level (21.2±3.0 ng/ml, n=10). In contrast, plasma cortisol concentrations did not change during the 5-hr experimental period in controls injected with saline. Thus, the increases after ACTH injection were significant at all time points compared with the time controls. The StAR mRNA content in the head kidney increased gradually after ACTH injection, and the increase was significant at 1.5 and 4.5 hr post-injection compared with that of saline-injected controls.

Fig. 4

Effect of ACTH injection on the levels of plasma cortisol and StAR mRNA in head kidney of freshwater eels. A, The plasma cortisol levels before and 0.5, 1.5, 4.5 h after ACTH injection were measured by enzyme immunoassay (EIA). Injection was made at 0hr. B, StAR mRNA expression in the head kidney at 1.5 and 4.5 hr post-injection was examined by RT-PCR. After electrophoresis, the StAR transcripts were quantitated and normalized to GAPDH levels. Values are means±SEM. Number of eels used for StAR mRNA quantitation was 5; that for cortisol measurement was 10 at 0, 0.5 and 1.5 hr post-injection, and 5 at 4.5 hr post-injection. Significant differences from control values at each time point are denoted by asterisks: *P<0.05; **P<0.01.

i0289-0003-20-2-211-f04.gif

Effects of SW transfer on plasma cortisol and Na+, and StAR mRNA in head kidney

Plasma cortisol concentration increased at 3 and 24 hr after transfer of eels from FW to SW (Fig. 5A). However, the plasma cortisol levels in FW-FW groups had no obvious increase, indicating that the transfer itself did not cause stress-induced cortisol production. For examination of plasma Na+ and StAR expression in head kidney, therefore, time controls were not prepared. As shown in Fig. 5B, plasma Na+ concentration was elevated at 3 and 24 hr after SW transfer, and the value at 24 hr was also significantly higher than that at 3 hr. However, the StAR content in head kidney was not significantly different between FW and SW-transferred eels (Fig. 5C).

Fig. 5

Effect of seawater transfer on plasma cortisol (A) and Na+ (B) concentration, and StAR mRNA content in head kidney (C) in eels. StAR transcripts were quantitated by RT-PCR and normalized to GAPDH levels. Values are means±SEM (n=6 for each group). Significant differences from the FW-FW controls are denoted by *P<0.05, ***P<0.001.

i0289-0003-20-2-211-f05.gif

Comparison of expression of two different StAR transcripts

Prior to the comparison of expression of the two transcripts with different length of 3′-UTR, we confirmed that StAR mRNA was expressed in all eels (data not shown), using a primer pair (S3-A3) that amplified the coding region of StAR (Fig. 1). Then, the difference in expression of the two transcripts was examined by the size of amplified products using the primer pair S2-A4 that could amplify the whole 3′-UTR (Figs. 1 and 6). Among 18 eels examined, a single band corresponding to the longer transcript was observed only in one eel, while a single band corresponding to the shorter transcript was detected in thirteen eels. In 4 of 18 eels, both transcripts were expressed in the head kidney. No obvious differences in relative abundance of the two transcripts were obtained between FW and SW-transferred eels (data not shown).

DISCUSSION

In this study, two StAR cDNAs differing in the length of 3′-UTR have been cloned from the head kidney of Japanese eel. The eel StAR is composed of 285 amino acid residues, which is identical or similar in length to those of teleosts and mammals thus far identified. The eel peptide displays 82.6% similarity to that of trout, and 67.1% to human. Compared with the StARs of other vertebrate species, the putative phosphorylation sites by protein kinase A (RRSS) (Strauss et al., 1999) are conserved in eel (Fig. 2). In the N-terminal 25 residues, eel StAR displays 96% similarity to that of trout or zebrafish, and 84% to that of human, rat or chicken. This domain is composed of basic and hydrophobic amino acids that are characteristic of mitochondrial targeting sequences (Clark et al., 1994). In the C-terminal domain, the amino acid residues believed to be important for the steroidogenic function (Watari et al., 1997), and those contributing to the hydrophobic tunnel structure for lipid transport (Tsujishita and Hurley, 2000), are also conserved (Fig. 2). These data indicate that the primary structure of StAR, particularly in the functional domain, is highly conserved throughout vertebrates.

The tissue distribution of eel StAR mRNA in the head kidney and gonads is in agreement with the reports of other species where StAR is principally expressed in steroidogenic tissues (Sugawara et al., 1995; Bauer et al., 2000; Kusakabe et al., 2002). Weak but distinct expression of StAR was also detected in the brain of eel, as well as in the rat and marmoset (Furukawa et al., 1998; Bauer et al., 2000). Recently, it is reported that various neurosteroids are produced locally in the brain and play diverse functions (Tsutsui et al., 2000). The expression of StAR in steroidogenic tissues and brain is consistent with the role of StAR in the regulation of steroidogenesis (Stocco, 2001). Although StAR transcripts were also detected in the kidney of human (Sugawara et al., 1995) and in some nonsteroidogenic tissues of trout (Kusakabe et al., 2002), the role of StAR in these tissues remains to be clarified.

Different lengths of StAR mRNAs have been reported in most species examined thus far. In some species, the difference in length can be attributable to the difference in the length of 3′-UTR (Fleury et al., 1998; Kerban et al., 1999). In bovine and rat StAR, multiple polyadenylation signals were found in the 3′-UTR, and it was suggested that different transcript sizes might represent the differential use of polyadenylation signals (Hartung et al., 1995; Pilon et al., 1997). In this study, two StAR transcripts differing in the length of 3′-UTR were identified in the eel. Since the longer mRNA contained two possible polyadenylation signals, while the shorter one lacks the first polyadenylation signal found in the longer one. This indicates that the shorter one was not generated by the use of the first polyadenylation signal. It is quite possible that the two mRNAs were generated by the alternative splicing from the same StAR gene, although we cannot exclude the possibility that they were encoded by different genes. The expression of the two StAR transcripts differed profoundly among eel individuals (Fig. 6). The reason and possible biological significance of two types of transcripts remain unknown.

Fig. 6

Comparison of the two different StAR transcripts in freshwater- and seawater-transferred eels. The expression of the two different StAR transcripts in the head kidney was examined by RT-PCR using primers S2 and A4 (Fig. 1), which could amplify the two transcripts with different length of 3′-UTR. Among the 18 fresh water and seawater-transferred eels examined, a band corresponding to the 1451 bp transcript was detected in 1 eel (lane 1), that corresponding to the 1111 bp transcript was detected in 13 eels (lane 2), both bands were detected in 4 eels (lane 3). M: 123 bp DNA marker.

i0289-0003-20-2-211-f06.gif

In non-mammalian vertebrates, the induction of StAR expression by trophic hormones has not yet been demonstrated except for an in vitro study using the follicular cells of the hen (Johnson and Bridgham, 2001). In this study, we showed that both plasma cortisol and StAR mRNA levels in the head kidney were significantly enhanced at 1.5 and 4.5 hr after ACTH injection. The close relationship between the increase of StAR expression and cortisol production strongly suggests that StAR is involved in the ACTH-induced cortisol production in eels as has been demonstrated in mammals (Kim et al., 1997; Stocco, 2001). At present, although we do not know the StAR mRNA content in the head kidney at 0.5 hr after ACTH injection, the results showed that the StAR mRNA content increased from 1.5 to 4.5 hr after ACTH injection. These results are, to some extent, similar to those in mammals, where peak increase of StAR mRNA levels usually occurred at 3–6 hr after ACTH treatment (LeHoux et al., 1998; Le Roy et al., 2000). Since the plasma cortisol level increased immediately after ACTH injection (within 0.5 hr, Fig. 4), it seems that the transcriptional and translational regulation of StAR may not be directly involved in the initial acute cortisol production as observed in rats, where the expression of StAR mRNA and protein was delayed after the peak increase in plasma corticosterone concentration (Ariyoshi et al., 1998). Epstein and Orme-Johnson (1991) proposed that a labile pool of StAR could be responsible for this acute mediation. It is also possible that redistribution of StAR rather than its net synthesis is critical for the steroido-genesis (Ariyoshi et al., 1998).

SW adaptation is a complex physiological process, in which cortisol plays a critical role by remodeling chloride cells and up-regulating the expression/activity of Na+, K+ATPase (McCormick, 1995). In the present study, after the transfer of eels from FW to SW, plasma Na+ concentration increased for 24 hr after transfer (Fig. 5). Thus plasma cortisol that increased in parallel appears to counteract the sudden increase in plasma Na+ concentration and to promote SW adaptation. The increase in plasma cortisol remained until 24 hr after SW transfer, this suggested that the chronic regulation, but not the acute regulation, of cortisol production might be prevailing during SW adaptation. In contrast, StAR mRNA content in the head kidney had no obvious increase, suggesting that the transcriptional regulation of StAR might not be directly involved in the regulation of cortisol production after SW transfer. This is not surprising, because StAR is mainly involved in the regulation of acute steroid production (Stocco, 2001). Besides, in addition to cortisol, multiple hormones such as growth hormone/insulin-like growth factor I axis, thyroid hormones, ANP, ANG II and urotensins are also implicated in SW adaptation, and some of them have been shown to increase cortisol production in eels and other teleost fishes (Arnold-Reed and Balment, 1994; McCormick, 2001; Tsukada and Takei, 2001; Li and Takei, 2003; Takei and Hirose 2002). Actually, plasma ANG II and ANP concentrations increased transiently after SW transfer in eels (Tierney et al., 1995; Kaiya and Takei, 1996). In mammals, it has been shown that the chronic regulation of trophic hormones, such as ACTH and ANG II, on the production of corticosteroids is largely mediated by increasing the transcription of steroidogenic enzymes (Hanukoglu, 1992; LeHoux et al., 1998; Le Roy et al., 2000). Therefore, it is reasonable that the increased cortisol production after SW transfer in eels might be mainly due to the enhanced expression of steroidogenic enzymes, under the stimulation of hormones such as ACTH, ANP and ANG II. This can be clarified in the near future since the cDNAs encoding the cytochrome P450 11β-hydroxylase (Jiang et al., 1996), 17α-hydroxylase (Kazeto et al., 2000), and 21-hydroxylase (Li et al., 2003), all of which are involved in cortisol biosynthesis, have already been cloned in the eel.

Acknowledgments

We thank Dr. Christopher A. Loretz of State University of New York at Buffalo for critical reading of this manuscript, and Ms. S. Hasegawa of Ocean Research Institute for help in experiment. This work was supported by grants-in-aid for Specially Promoted Grant (01902008) and for Creative Basic Research (12NP0201) from the Ministry of Education, Science, Sports and Culture of Japan and for Scientific Research (A) (13304063) from Japan Society for the Promotion of Science to Y. T. Y.-Y. Li is a recipient of Postdoctoral Fellowship from Japan Society for the Promotion of Science.

REFERENCES

1.

N. Ariyoshi, Y. C. Kim, I. Artemenko, K. K. Bhattacharya, and C. R. Jefcoate . 1998. Characterization of the rat StAR gene that encodes the predominant 3.5 kb mRNA: ACTH stimulation of adrenal steroids in vivo precedes elevation of StAR mRNA and protein. J Biol Chem 273:7610–7619. Google Scholar

2.

D. E. Arnold-Reed and R. J. Balment . 1994. Peptide hormones influence in vitro interrenal secretion of cortisol in the trout, Oncorhynchus mykiss. Gen Comp Endocrinol 96:85–91. Google Scholar

3.

M. P. Bauer, J. T. Bridgham, D. M. Langenau, A. L. Johnson, and F. W. Goetz . 2000. Conservation of steroidogenic acute regulatory (StAR) protein structure and expression in vertebrates. Mol Cell Endocrinol 168:119–125. Google Scholar

4.

B. J. Clark, J. Wells, S. R. King, and D. M. Stocco . 1994. The purification, cloning, and expression of a novel luteinizing hormone-induced mitochondrial protein in MA-10 mouse Leydig tumour cells. Characterization of the steroidogenic acute regulatory protein (StAR). J Biol Chem 269:28314–28322. Google Scholar

5.

D. Dewied 1990. Neurotrophic effects of ACTH/MSH neuropep-tides. Acta Neurobiol Exp 50:353–366. Google Scholar

6.

L. F. Epstein and N. R. Orme-Johnson . 1991. Regulation of steroid hormone biosynthesis: identification of precursors of a phosphoprotein targeted to the mitochondrion in stimulated rat adrenal cortex cells. J Biol Chem 266:19739–19745. Google Scholar

7.

A. Fleury, L. Ducharme, and J. G. LeHoux . 1998. in vivo effects of adrenocorticotrophin on the expression of the hamster steroidogenic acute regulatory protein. J Mol Endocrinol 21:131–139. Google Scholar

8.

J. N. Forrest, W. C. MacKay, B. Gallagher, and F. H. Epstein . 1973. Plasma cortisol response to saltwater adaptation in the American eel Anguilla rostrata. Am J Physiol 224:714–717. Google Scholar

9.

A. Furukawa, A. Miyatake, T. Ohnishi, and Y. Ichikawa . 1998. Steroidogenic acute regulatory protein (StAR) transcripts constitutively expressed in the adult rat central nervous system: colocalization of StAR, cytochrome P-450scc (CYP X1A1), and 3β-hydroxysteroid dehydrogenase in the rat brain. J Neurochem 71:2231–2238. Google Scholar

10.

I. Hanukoglu 1992. Steroidogenic enzymes: structure, function, and role in regulation of steroid hormone biosynthesis. J Steroid Biochem Mol Biol 43:779–804. Google Scholar

11.

S. Hartung, W. Rust, M. Balvers, and R. Ivell . 1995. Molecular cloning and in vivo expression of the bovine steroidogenic acute regulatory protein. Biochem Bioph Res Co 215:646–653. Google Scholar

12.

I. W. Henderson, V. Jotisankasa, W. Mosley, and M. Oguri . 1976. Endocrine and environmental influences upon plasma cortisol concentrations and plasma rennin activity of the eel, Anguilla anguilla L. J Endocrinol 70:81–95. Google Scholar

13.

K. Inoue, M. J. Russel, K. R. Olson, and Y. Takei . 2003. C-type natriuretic peptide of rainbow trout (Oncorhynchus mykiss): primary structure and vasorelaxant activities. Gen Comp Endocrinol in press. Google Scholar

14.

J. Q. Jiang, T. Kobayashi, W. Ge, H. Kobayashi, M. Tanaka, M. Okamoto, Y. Nonaka, and Y. Nagahama . 1996. Fish testicular 11β-hydroxylase: cDNA cloning and mRNA expression during spermatogenesis. FEBS Lett 397:250–252. Google Scholar

15.

A. L. Johnson and J. T. Bridgham . 2001. Regulation of steroidogenic acute regulatory protein and luteinizing hormone receptor messenger ribonucleic acid in hen granulosa cells. Endocrinology 142:3116–3124. Google Scholar

16.

H. Kaiya and Y. Takei . 1996. Atrial and ventricular natriuretic peptide concentrations in plasma of freshwater- and seawater-adapted eels. Gen Comp Endocrinol 102:183–190. Google Scholar

17.

Y. Kazeto, S. Ijiri, T. Todo, S. Adachi, and K. Yamauchi . 2000. Molecular cloning and characterization of Japanese eel ovarian P450c17 (CYP17) cDNA. Gen Comp Endocrinol 118:123–133. Google Scholar

18.

A. Kerban, D. Boerboom, and J. Sirois . 1999. Human chorionic gonadotropin induces an inverse regulation of steroidogenic acute regulatory protein messenger ribonucleic acid in theca interna and granulosa cells of equine preovulatory follicles. Endocrinology 140:667–674. Google Scholar

19.

Y. C. Kim, N. Ariyoshi, I. Artemenko, M. E. Elliott, K. K. Bhattacharyya, and C. R. Jefcoate . 1997. Control of cholesterol access to cytochrome P450scc in rat adrenal cells mediated by regulation of the steroidogenic acute regulatory protein. Steroids 62:10–20. Google Scholar

20.

M. Kusakabe, T. Todo, H. J. McQuillan, F. W. Goetz, and G. Young . 2002. Characterization and expression of steroidogenic acute regulatory protein and MLN64 cDNAs in trout. Endocrinology 143:2062–2070. Google Scholar

21.

J. G. LeHoux, A. Fleury, and L. Ducharme . 1998. The acute and chronic effects of adrenocorticotropin on the levels of messenger ribonucleic acid and protein of steroidogenic enzymes in rat adrenal in vivo. Endocrinology 139:3913–3922. Google Scholar

22.

C. Le Roy, J. Y. Li, D. M. Stocco, D. Langlois, and J. M. Saez . 2000. Regulation by adrenocorticotropin (ACTH), angiotensin II, transforming growth factor-fl, and insulin-like growth factor I of bovine adrenal cell steroidogenic capacity and expression of ACTH receptor, steroidogenic acute regulatory protein, cytochrome P450c17, and 3β-hydroxysteroid dehydrogenase. Endocrinology 141:1599–1607. Google Scholar

23.

Y-Y. Li and Y. Takei . 2003. Ambient salinity-dependent effects of homologous natriuretic peptides (ANP, VNP and CNP) on plasma cortisol level in the eel. Gen Comp Endocrinol in press. Google Scholar

24.

Y-Y. Li, K. Inoue, and Y. Takei . 2003. Interrenal steroid 21-hydroxylase in eels: primary structure, progesterone-specific activity and enhanced expression by ACTH. J Mol Endocrinol in press. Google Scholar

25.

S. D. McCormick 1995. Hormonal control of gill Na+, K+-ATPase and chloride cell function. In “Cellular and Molecular Approaches to Fish Ionic Regulation”. Ed by C. M. Wood and T. J. Shuttleworth . Academic Press. San Diego. pp. 285–316. Google Scholar

26.

S. D. McCormick 2001. Endocrine control of osmoregulation in teleost fish. Am Zoologist 41:781–794. Google Scholar

27.

W. L. Miller 1988. Molecular biology of steroid hormone synthesis. Endocr Rev 9:295–318. Google Scholar

28.

N. Pilon, I. Daneau, C. Brisson, J. F. Euthier, J. G. Lussier, and D. W. Silversides . 1997. Porcine and bovine steroidogenic acute regulatory protein (StAR) gene expression during gestation. Endocrinology 138:1085–1091. Google Scholar

29.

D. M. Stocco 2001. StAR protein and the regulation of steroid hormone biosynthesis. Ann Rev Physiol 63:193–213. Google Scholar

30.

J. F. Strauss III, C. B. Kallen, L. K. Christenson, H. Watari, L. DeVoto, F. Ara-kane, M. Kiriakidou, and T. Sugawara . 1999. The steroidogenic acute regulatory protein (StAR): a window into the complexities of intracellular cholesterol trafficking. Recent Prog Horm Res 54:369–395. Google Scholar

31.

T. Sugawara, J. A. Holt, D. Driscoll, J. F. Strauss III, D. Lin, W. L. Miller, D. Patterson, K. P. Clancy, I. M. Hart, B. J. Clark, and D. M. Stocco . 1995. Human steroidogenic acute regulatory protein: functional activity in COS-1 cells, tissue-specific expression, and mapping of the structural gene to 8p11.2 and a pseudogene to chromo-some 13. Proc Natl Acad Sci USA 92:4778–4782. Google Scholar

32.

Y. Takei 1993. Role of peptide hormones in fish osmoregulation. In “Fish Ecophysiology”. Ed by C. Rankin and F. B. Jensen . Chapman & Hall. London. pp. 136–160. Google Scholar

33.

Y. Takei and S. Hirose . 2002. The natriuretic peptide system in eels: a key endocrine system for euryhalinity? Am J Physiol 282:R940–R951. Google Scholar

34.

Y. Takei, K. Inoue, K. Ando, T. Ihara, T. Katafuchi, M. Kashiwagi, and S. Hirose . 2001. Enhanced expression and release of C-type natriuretic peptide in freshwater eels. Am J Physiol 280:R1727–R1735. Google Scholar

35.

M. L. Tierney, G. Cramb, and N. Hazon . 1995. Stimulation of the reninangiotensin system and drinking by papaverine in the seawater eel, Anguilla anguilla. J Fish Biol 46:721–724. Google Scholar

36.

Y. Tsujishita and J. H. Hurley . 2000. Structure and lipid transport mechanism of a StAR-related domain. Nat Struct Biol 7:408–414. Google Scholar

37.

T. Tsukada and Y. Takei . 2001. Relative potency of three homologous natriuretic peptides (ANP, CNP and VNP) in eel osmoregulation. Zool Sci 18:1253–1258. Google Scholar

38.

K. Tsutsui, K. Ukena, M. Usui, H. Sakamoto, and M. Takase . 2000. Novel brain function: biosynthesis and actions of neurosteroids in neurons. Neurosci Res 36:261–273. Google Scholar

39.

H. Watari, F. Arakane, C. Moog-Lutz, C. B. Kallen, C. Tomasetto, G. L. Gerton, M. C. Rio, M. E. Baker, and J. F. Strauss III . 1997. MLN64 contains a domain with homology to the steroidogenic acute regulatory protein (StAR) that stimulates steroidogenesis. Proc Natl Acad Sci USA 94:8462–8467. Google Scholar
Yuan-You Li, Koji Inoue, and Yoshio Takei "Steroidogenic Acute Regulatory Protein in Eels: cDNA Cloning and Effects of ACTH and Seawater Transfer on Its mRNA Expression," Zoological Science 20(2), 211-219, (1 February 2003). https://doi.org/10.2108/zsj.20.211
Received: 13 September 2002; Accepted: 1 November 2002; Published: 1 February 2003
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