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J Clin Invest. Jun 1, 2009; 119(6): 1647–1658.
Published online May 11, 2009. doi:  10.1172/JCI35314
PMCID: PMC2689130

Tonicity-dependent induction of Sgk1 expression has a potential role in dehydration-induced natriuresis in rodents


In various mammalian species, including humans, water restriction leads to an acute increase in urinary sodium excretion. This process, known as dehydration natriuresis, helps prevent further accentuation of hypernatremia and the accompanying rise in extracellular tonicity. Serum- and glucocorticoid-inducible kinase (Sgk1), which is expressed in the renal medulla, is regulated by extracellular tonicity. However, the mechanism of its regulation and the physiological role of hypertonicity-induced SGK1 gene expression remain unclear. Here, we identified a tonicity-responsive enhancer (TonE) upstream of the rat Sgk1 transcriptional start site. The transcription factor NFAT5 associated with TonE in a tonicity-dependent fashion in cultured rat renal medullary cells, and selective blockade of NFAT5 activity resulted in suppression of the osmotic induction of the Sgk1 promoter. In vivo, water restriction of rats or mice led to increased urine osmolality, increased Sgk1 expression, increased expression of the type A natriuretic peptide receptor (NPR-A), and dehydration natriuresis. In cultured rat renal medullary cells, siRNA-mediated Sgk1 knockdown blocked the osmotic induction of natriuretic peptide receptor 1 (Npr1) gene expression. Furthermore, Npr1–/– mice were resistant to dehydration natriuresis, which suggests that Sgk1-dependent activation of the NPR-A pathway may contribute to this response. Collectively, these findings define a specific mechanistic pathway for the osmotic regulation of Sgk1 gene expression and suggest that Sgk1 may play an important role in promoting the physiological response of the kidney to elevations in extracellular tonicity.


Persistent hypertonicity, typically reflecting a high extracellular sodium concentration, stresses mammalian cells due to the ensuing osmotic efflux of water that shrinks the cells and concentrates their contents. Under most conditions, the concentration of extracellular sodium in mammals is controlled primarily through regulation of water metabolism. As extracellular sodium and plasma tonicity rise, the thirst mechanism is activated, and secretion of the neurohypophyseal hormone vasopressin into plasma increases. Vasopressin binds to its cognate receptors in the collecting duct of the kidney, resulting in increased water retention.

Following short-term water restriction, several mammals demonstrate an acute increase in urinary sodium excretion that is independent of changes in water metabolism. This response, termed dehydration natriuresis (111), plays an important role in preventing further accentuation of hypernatremia and the accompanying rise in extracellular tonicity. A similar natriuresis is seen following infusion of hypertonic saline (12). Investigations to date have suggested a role for central versus peripheral osmoreceptors and blood-borne versus neural effectors in contributing to dehydration-induced natriuresis; however, the precise mechanism(s) underlying this natriuresis remains undefined.

Changes in renal medullary tonicity have been shown to regulate the expression of a variety of genes, including those encoding aldose reductase (13), the betaine/GABA transporter (14), taurine transporter (TauT) (15), HSP-70 (16), the sodium/myo-inositol cotransporter (17), the urea transporters (18), and aquaporin 2 (19), expression of all of which increases in response to increased extracellular tonicity. In each case, the increase in gene expression has been traced to an increase in gene transcription that is mediated through a TonE (TGGAAANNNCN, where N is any nucleotide positioned in the promoter of the target gene) (14, 20). The TonE-binding protein (TonEBP) is a dimeric protein that associates with the TonE in asymmetric fashion, effectively encircling its recognition element in the target gene promoter (21). Dimerization is not tonicity dependent, but it is required for DNA binding and activation of the transcription factor (22). TonEBP has subsequently been identified as a distant relative of the nuclear factor of activated T cells (NFAT) nuclear transcription factor family (i.e., it shares 43% sequence identity with NFAT1) and assigned the name NFAT5 (23). In the basal state, TonEBP/NFAT5 is distributed in both the nucleus and cytoplasm of the cell. Following exposure to a hypertonic environment in vitro (24, 25) or water restriction in vivo (26), it translocates selectively into the nuclear compartment. Hypertonicity also increases NFAT5 gene expression, albeit with a delayed time course (27, 28).

Each of the NFAT5-mediated osmosensitive genes mentioned above, in one way or another, generates products or activates signaling pathways that function in a counterregulatory fashion to mitigate the impact of the hypertonic stimulus. Most of the changes are, in fact, passive adaptive reactions to protect cells from hypertonic damage. To date, few tonicity-induced genes that possess the capacity to reduce hypertonicity per se, and none linked to dehydration natriuresis, have been identified.

Serum- and glucocorticoid-regulated kinase 1 (Sgk1) is a signaling kinase that is induced by a variety of stimuli, including serum (29), glucocorticoids (29, 30), TGF-β (31, 32), aldosterone (33), and hypertonicity (3438). The mechanism and the underlying physiological function of hypertonicity-induced SGK1 gene expression remain unclear. We have shown previously that Sgk1, which is avidly expressed in the renal medulla (39), is stimulated by increased extracellular tonicity in inner medullary collecting duct (IMCD) cells of the kidney (40). We have also demonstrated that hypertonicity increases expression of the type A natriuretic peptide receptor (NPR-A) (41), a guanylyl cyclase–linked receptor that binds both atrial natriuretic peptide (ANP) and the B-type natriuretic peptide (BNP), leading to an increase in renal excretion of sodium. Water deprivation leads to increased renal medullary sodium concentration (4, 42, 43). We reasoned that tonicity-dependent stimulation of Sgk1 and subsequent activation of NPR-A gene expression might be linked to the dehydration natriuresis described above.

In the present study, we demonstrate that Sgk1 does indeed serve as an intermediary in tonicity-dependent stimulation of NPR-A gene expression and that dehydration-induced natriuresis is linked to increased expression of Sgk1 and NPR-A in rats and mice. Furthermore, dehydration-induced natriuresis does not occur in NPR-A gene–deleted (Npr1–/–) mice. The osmotic induction of Sgk1 gene expression in IMCD cells is associated with an increase in Sgk1 gene promoter activity, and this induction is critically dependent upon a single TonE site positioned between –324 and –312 bp upstream from the transcription start site in the gene. Interaction of NFAT5 with this TonE site is required for the hypertonic, but not the hypotonic, induction of the Sgk1 gene promoter. Collectively, these data suggest a role for Sgk1 and the intrinsic renal natriuretic peptide system as contributors to the phenomenon of dehydration-induced natriuresis.


Like the Sgk1 gene transcript and the Sgk1 protein (40), Sgk1 promoter activity proved to be very responsive to increases in extracellular tonicity in IMCD cells. As shown in Figure Figure1A,1A, IMCD cells transfected with the Sgk promoter–driven luciferase reporter demonstrated a 5- to 6-fold increase in promoter activity following exposure to an approximately 150-mOsm/kg increase (i.e., above the tonicity of DMEM medium, which is 296 mOsm/kg H2O) in extracellular tonicity. The background vector (pGL3-Luc) showed no sensitivity to extracellular tonicity.

Figure 1
Osmotic induction of rat Sgk1 promoter in rat IMCD cells.

The osmotic activation of this promoter was dependent on the p38 MAPK signaling system (Figure (Figure1B).1B). Treatment of the IMCD cells with the p38 MAPK inhibitor SB203580 led to a dose-dependent suppression of the osmotic induction of Sgk1-Luc reporter activity. Similarly, cotransfection with a dominant negative mutant of MKK6, an activating kinase immediately upstream from p38 MAPK (41), resulted in a nearly 50% decrease in the tonicity-dependent induction.

Earlier studies (34) indicated that osmotic induction of the Sgk1 promoter in NMuMg cells is dependent on a GC-rich region, shown in vitro to associate with the transcription factor Sp1, in close proximity to the transcription start site of the Sgk1 gene. Since Sp1-binding sites have not been linked to induction of osmotically sensitive genes in renal cells, we examined the promoter sequence for the presence of alternative sites that might contribute to the osmotic induction. We identified a consensus tonicity-responsive enhancer (TonE) (44) approximately 312 bp upstream from the transcription start site. The rat Sgk1 TonE (TGGAAAATCACC) (Figure (Figure2A)2A) is completely homologous with the murine and human aldose reductase osmoregulatory elements (13, 45). We introduced a series of point mutations into the putative TonE in the Sgk1 promoter–driven luciferase reporter and transfected these into IMCD cells. As shown in Figure Figure2B,2B, one of the mutations (M3) led to complete reversal of the osmotic induction, while 2 of the others, M1 and M2, led to intermediate levels of inhibition; a fourth, M4, with base modifications outside the core TonE, was without effect.

Figure 2
Mutation of TonE blocks osmotic induction of the Sgk1 gene promoter in IMCD cells.

Given the previous association of the putative Sp1-binding element (34) with the osmotic induction of this promoter’s activity, we created a mutation in this site, alone and in combination with the TonE mutation (Figure (Figure3A),3A), and introduced the reporters into IMCD cells. As shown in Figure Figure3B,3B, virtually the entire osmotic induction appears to flow through TonE in these cells. Mutation of the Sp1-binding element in the GC-rich region did not affect the osmotic induction when tested alone or in the presence of the TonE mutation. Thus, while this Sp1-binding element appears to play a role in controlling the Sgk1 promoter response to tonicity in NMuMg cells (34), in IMCD cells the TonE site dominates in orchestrating this response.

Figure 3
Proximal Sp1-binding elements do not participate in the osmotic induction of Sgk1 promoter activity in rat IMCD cells.

In the case of the aldose reductase (13) and betaine transporter (20) genes, a specific nuclear transcription factor termed NFAT5 has been shown to associate with TonE and stimulate transcriptional activity of the contiguous promoter. To explore the involvement of NFAT5 as a mediator of the osmotic induction of the Sgk1 promoter, we carried out EMSA of nuclear extracts from IMCD cells cultured under isotonic versus hypertonic (NaCl) conditions using radiolabeled Sgk1 TonE sequence as a probe. As shown in Figure Figure4A,4A, exposure to the hypertonic environment resulted in an increase in protein association with the oligonucleotide harboring the TonE, here designated as the NFAT5 complex. Incubation with anti-NFAT5 antibody, but not with antibody directed against the p50 subunit of NF-κB, resulted in a supershift of the associated protein. The NFAT5 complex was competed by unlabeled oligonucleotide harboring the wild-type sequence and by the sequence harboring the M4 mutation, but not by oligonucleotides harboring mutations M1, M2, or M3 (Figure (Figure4B).4B). Thus, the relative affinity of NFAT5 for these mutated osmotic response element (ORE) sequences mirrors the ability of these sequences to signal the osmotic induction of the Sgk1 promoter (see Figure Figure2). 2).

Figure 4
NFAT5 binding to TonE in the Sgk1 promoter in vitro.

Western blot analysis for NFAT5 protein showed that there was a shift of protein from the cytoplasm into the nuclear compartment after 4 hours of exposure to the hypertonic environment (75 mM NaCl), and this nuclear sequestration persisted for 24 hours (Figure (Figure4,4, C and D). In addition, there was a net increase in levels of total NFAT5 protein at 24 hours that was not present at the 4-hour time point (Figure (Figure4E). 4E).

To confirm that the osmotically dependent NFAT5 association with the Sgk1 promoter takes place within the context of the intact cell, we carried out ChIP analysis of the endogenous rat Sgk1 promoter using an antibody directed against NFAT5. As shown in Figure Figure5A,5A, exposure of IMCD cells to hypertonic medium (addition of 75 mM NaCl or 150 mM sucrose to culture medium) led to increased association of both NFAT5 and RNA polymerase II with the native Sgk1 gene relative to the isotonic control. Neither NFAT5 nor RNA polymerase II interacted to any significant degree with sequence lacking the TonE positioned 3.2 kb upstream from the Sgk1 gene. To prove that this interaction between NFAT5 and the Sgk1 gene promoter requires the TonE-binding sequence described above, we introduced reporter plasmids harboring 1,474 bp of rat Sgk1 5′ flanking sequence (–1,430 to +44) into IMCD cells by transient transfection. One of these reporters contained entirely wild-type sequence, while the other harbored a selective mutation (M3) in the TonE. As shown in Figure Figure5B,5B, the wild-type sequence showed evidence of substantial osmosensitive association with NFAT5 in the ChIP assay; mutation of the TonE-binding site resulted in near complete loss of this association.

Figure 5
ChIP analysis of the Sgk1 promoter.

To link the NFAT5 protein functionally to the osmotic induction of Sgk1 promoter activity, we used 2 different approaches to inhibit NFAT5 activity. Introduction of U6-N5 ex8, a small inhibitory RNA vector that specifically targets the NFAT5 endogenous transcript (46), completely reversed the osmotic induction of the Sgk1 promoter, while the empty U6 vector was devoid of activity (Figure (Figure6).6). Similarly, introduction of a dominant negative NFAT5 expression vector (NFAT5-DN) along with the Sgk1-Luc reporter led to significant inhibition of the osmotic response. Collectively, these findings, along with the results presented above, support the hypothesis that NFAT5 is the relevant transcription factor that binds to the Sgk1 TonE and mediates the osmotic induction of that gene’s promoter in IMCD cells.

Figure 6
Selective inhibition of NFAT5 leads to blockade of the hypertonic induction of the Sgk1 gene promoter.

A previous study by Rozansky et al. (47) demonstrated that sgk1 gene expression can also be activated by reductions in extracellular tonicity (i.e. hypoosmolality) in A6 cells. To evaluate this phenomenon in cultured IMCD cells and its dependence on the TonE site described above, we introduced the wild-type Sgk1-Luc or the TonE-mutated Sgk1-Luc into primary cultures of rat IMCD cells and exposed them to either a hyper- or a hypotonic environment. As shown in Figure Figure7,7, relative to the cells cultured in isotonic medium, cells exposed to either the hypo- or hypertonic medium showed a significant increase in expression of the wild-type Sgk1 promoter. However, while mutation of the TonE, as expected, led to a near complete inhibition of the hypertonic stimulation of promoter activity, it had virtually no effect on the hypotonic stimulation. This implies that the hypotonic stimulation of Sgk1 gene transcription operates over signaling pathways that are largely independent of those used for the hypertonic induction, including NFAT5 and the TonE.

Figure 7
Hypotonic induction of the Sgk1 promoter does not require TonE.

As mentioned above, expression of both Sgk1 and NPR-A has been shown to increase in IMCD cells exposed to increased extracellular tonicity. To establish the link between Sgk1 and the induction of NPR-A gene expression, we employed an siRNA approach. Cultured rat IMCD cells were transfected with one of 3 siRNA sequences, each of which was designed to target the rat Sgk1 gene coding sequence, prior to exposure of the cells to increased extracellular tonicity (75 mM NaCl). As shown in Figure Figure8A,8A, exposure to hypertonic culture media resulted in a 4- to 5-fold increase in Sgk1 mRNA expression in these cells. This increment was partially reduced by siSgk1A and siSgk1B and nearly completely eliminated by cotransfection with siSgk1C. Similarly, as shown in the Western blot in Figure Figure8B,8B, siSgk1C had little effect on basal levels of Sgk1 protein, but it nearly completely reversed the NaCl-dependent increment in Sgk1. The same level of extracellular tonicity (75 mM NaCl) led to a 3-fold increase in NPR-A mRNA levels (Figure (Figure8C)8C) and a 4-fold increment in NPR-A protein levels (Figure (Figure8D)8D) in IMCD cells. Transfection of these cells with siSGK1C inhibited the increase in NPR-A protein and mRNA by approximately 60%. Collectively, these data indicate that the osmotic induction of Sgk1 is a major contributor to the osmotic stimulation of NPR-A gene expression in IMCD cells.

Figure 8
Sgk1 siRNA blocks NaCl-induced Sgk1 and NPR-A gene transcription and translation.

To extend this observation to an in vivo model, we subjected male Sprague-Dawley rats to 24 hours of water deprivation, a procedure that is known to increase urine osmolality (4, 8, 10, 26, 43) and renal medullary sodium concentration (4, 42, 43). As shown in Table Table1,1, water deprivation resulted in a significant increase in urine osmolality (~40% increase over the baseline urine osmolality). There was a modest, but not statistically significant, increase in plasma osmolality, and no significant change in systolic or diastolic blood pressure in these 2 groups. The water-restricted animals lost approximately 10% of their body weight over the 24-hour period, while weights in the control animals were stable.

Table 1
Effect of 24-hour water restriction on plasma aldosterone levels, plasma and urine osmolality, blood pressure, and body weight (before and after dehydration)

Water restriction was associated with a statistically significant increase in urinary sodium excretion (Figure (Figure9A),9A), confirming the presence of the dehydration natriuresis observed by others in rats, rabbits, sheep, mice, dogs, and humans (111) following short-term water restriction. This was accompanied by a significant increase in Sgk1 mRNA (Figure (Figure9B)9B) and Sgk1 protein (Figure (Figure9C)9C) in the renal IMCD. Because Sgk1 gene expression is known to be regulated by aldosterone, we measured plasma aldosterone levels at the end of the water deprivation period. As reported in Table Table1,1, there was no change in plasma aldosterone levels after 24-hour water deprivation, a finding that is consistent with previous dehydration studies (3, 9, 11). Since some studies (48, 49) have shown that increased Sgk1 expression is linked to increased epithelial sodium channel (ENaC) expression, we asked whether dehydration-induced Sgk1 expression was associated with increased ENaC expression. As shown in Figure Figure9D,9D, water restriction modestly increased expression of the α subunit of ENaC (αENaC). However, this modest elevation in αENaC expression was accompanied by increased sodium excretion rather than sodium absorption (see Figure Figure9A),9A), implying that Sgk1-mediated activation of natriuresis plays a dominant physiological role in this special circumstance.

Figure 9
Water restriction increases urine sodium excretion, Sgk1 mRNA, and protein levels in rat IMCD.

The increase in Sgk1 expression was accompanied by an increase in NPR-A mRNA (Figure (Figure10A)10A) and protein (Figure (Figure10B),10B), which, in turn, were linked to a 3-fold increase in urinary cyclic GMP excretion (Figure (Figure10C).10C). Cyclic GMP is the biological end product of NPR-A activation (i.e., ligand-dependent guanylyl cyclase activation).

Figure 10
Dehydration activates the natriuretic peptide system in rat IMCD.

To investigate a possible role for the ligand itself (i.e., ANP) in contributing to this increase in urinary cyclic GMP, we measured ANP mRNA transcript levels in the atria of the control versus water-restricted rats, as well as plasma ANP levels in the 2 groups. As shown in Figure Figure10,10, D and E, water restriction reduced, rather than increased, expression of the atrial ANP gene and circulating levels of ANP.

The kidney itself is also thought to be a source of ANP gene expression. Cells of the distal nephron have been shown to harbor proANP gene transcripts and ANP immunoreactivity (50), and ANP immunoreactivity has been identified in the urine (51). Urinary ANP, termed urodilatin, is a product of the renal ANP gene with a 4-amino-acid N-terminal extension (supplied from the proANP precursor) linked to the core ANP peptide (52). As shown in Figure Figure10F,10F, expression of proANP mRNA in the inner medulla is increased following 24 hours of water restriction, as is the excretion of urodilatin in urine (Figure (Figure10G)10G) (urodilatin concentration in urine: control, 4.37 ± 0.64 pg/μl vs. dehydrated, 9.33 ± 1.01 pg/μl; P < 0.01), suggesting that locally generated ligand as well as increased expression of the NPR-A receptor (see above) contribute to the increased urinary excretion of sodium in the acutely dehydrated state.

To confirm the mechanistic link between dehydration natriuresis and increased NPR-A expression, we examined the effect of 24-hour water restriction in wild-type and Npr1–/– (i.e., NPR-A gene–deleted) mice. As noted previously (53), Npr1–/– mice display significant hypertension compared with control littermates (systolic BP, 112.8 ± 10.6 vs. 103.8 ± 6.9 mmHg, P < 0.01; diastolic BP, 96.8 ± 12.5 vs. 83.3 ± 8.1 mmHg, P < 0.05). Twenty-four hours of water deprivation resulted in weight loss (12% in wild-type and 13% in Npr1–/– mice) and increased urine osmolality in wild-type and Npr1–/– mice compared with their respective control littermates with free access to water (wild-type, 3,123.4 ± 606.4 vs. 1,817.9 ± 401.5 mOsm/kg H2O, P < 0.01; Npr1–/–, 2,415.6 ± 549.1 vs. 1,568.8 ± 578.5 mOsm/kg H2O, P < 0.01). This was accompanied by a significant increase in Sgk1 protein expression in IMCD (Figure (Figure11A),11A), suggesting that hyperosmolality activates Sgk1 expression in this nephron segment in both wild-type and Npr1–/– mice. Urinary sodium excretion was markedly increased during 24 hours of water restriction in wild-type mice (Figure (Figure11B);11B); however, this natriuresis did not occur in Npr1–/– mice (Figure (Figure11B).11B). As expected, dehydration dramatically increased NPR-A expression in wild-type mice; there was no NPR-A protein expression in Npr1–/– mice (Figure (Figure11C).11C). NPR-A activity, assessed as urinary cyclic GMP excretion, was significantly increased in dehydrated wild-type but not in dehydrated Npr1–/– mice (Figure (Figure11D).11D). These findings support a mechanistic link between dehydration-induced natriuresis and NPR-A signaling activity.

Figure 11
Effect of water restriction on the Sgk1/NPR-A signaling pathway in wild-type and Npr1–/– mice.


The signaling kinase Sgk1 is known to be regulated by extracellular tonicity (3438). However, the mechanism underlying this regulation remains only partially understood. Previous studies by Bell et al. (34) using HMuMg mammary epithelial cells showed that Sgk1 gene promoter activity increased in response to extracellular hypertonicity; however, their results suggested that this increase was heavily dependent on a GC-rich segment of the proximal promoter that appeared to bind to the transcription factor Sp1. In our study, this particular Sp1 site or sites did not contribute greatly to the osmotic induction of Sgk1 in primary cultures of rat IMCD cells. Instead, virtually all of the osmoregulatory activity required the presence of an intact TonE element much further upstream in the promoter. The reason(s) behind this differential response remain undefined, but the data suggest that different cell types may use different mechanisms to forge the signal linking extracellular tonicity to the transcriptional machinery. HMuMg cells, as mammary epithelial cells, exist largely in an isotonic environment in their natural location in vivo, while IMCD cells are positioned in the medulla of the kidney. This region is subject to wide swings in extracellular tonicity, and it plays a key role in linking tonicity to physiological responses. It is possible, therefore, that IMCD cells have refined the osmoregulatory signals responsible for controlling Sgk1 gene expression beyond those available to mammary epithelial cells.

NFAT5 levels have been shown to increase in a linear fashion with increases in extracellular tonicity (54). Nuclear TonEBP is increased throughout the medulla in dehydrated versus water-loaded animals (26). It is noteworthy that Rozansky et al. showed that sgk1, in addition to being stimulated by increases in extracellular tonicity, is also stimulated by decreases in extracellular tonicity (47). The latter has been demonstrated using hypo-osmotic induction of A6 cells and confirmed here using rat IMCD cells. The biphasic response of the Sgk1 promoter would be difficult to explain using a single NFAT5-dependent regulatory mechanism, and in fact, our results suggest that only the response to hypertonicity is NFAT5/TonE dependent. This implies that the hypotonic induction of Sgk1 gene transcription operates independently of NFAT5 and the TonE.

Several genes have been shown to respond to extracellular tonicity with altered expression (55, 56). A significant number of these, including the betaine/GABA transporter gene (14), the sodium-myoinositol cotransporter gene (17), the heat shock protein HSP-70 gene (16), the urea transporters encoded by the UT-A gene (18), the TNF gene (46), the aquaporin 2 gene (19), and aldose reductase genes (13) respond through an NFAT5/TonEBP-binding element (TonE) in their respective promoters. Several of these exert counterregulatory activity that, at least in part, serves to dampen the effects of increased extracellular tonicity. The inositol and betaine transporters, for example, raise intracellular osmolality without increasing ionic strength, thereby protecting the cell from the damaging effects of the latter (14, 17). However, most of these gene products act passively to protect cells from hypertonicity. To date, no tonicity-induced genes have been identified that functionally feed back to increase the excretion of sodium, the dominant contributor to plasma tonicity. The demonstrated osmosensitivity of the Sgk1 gene promoter and the demonstration that this sensitivity is dependent upon an NFAT5-binding TonE element between –324 and –312 bp in the promoter supports the hypothesis that Sgk1 is a physiological target of extracellular tonicity in the IMCD. Sgk1 could, by analogy to the gene products listed above, function to dampen or inhibit the sequelae attendant to increased extracellular tonicity, as occurs with dehydration following water restriction. At the organismal level, this appears to involve increased activity of the natriuretic peptide system and enhanced urinary sodium excretion, an effect that would counter increased extracellular tonicity through reduction of extracellular solute levels.

Dehydration-induced natriuresis has been described in a variety of mammalian species including rats, rabbits, sheep, mice, dogs, and humans (111). It typically occurs within the first 24–48 hours following the onset of water restriction, presumably before significant contraction of intravascular volume has occurred. It is characterized by a moderate increase in urinary sodium excretion that gradually wanes as volume contraction and mechanisms associated with increased renal sodium retention come to dominate the physiology. The mechanism underling this natriuresis remains unclear. Data have been presented suggesting that the neurohypophyseal hormone oxytocin may participate in this natriuresis. Levels of plasma oxytocin increase slightly in water-restricted states, concomitant with the natriuresis (2). However, oxytocin infusion in humans placed on either a high- or low-salt diet proved incapable of producing natriuresis (57).

We have shown previously that increased extracellular tonicity leads to an increase in NPR-A gene expression and NPR-A activity (41), with concomitant increased expression of Sgk1 (40). We have hypothesized that it is Sgk1 that mediates the increase in NPR-A expression, a hypothesis that draws strength from the siRNA studies presented here. Under conditions where the osmotic induction of Sgk1 gene expression in IMCD cells is almost completely suppressed by an appropriately targeted siRNA, there is a parallel reduction in NPR-A gene expression. This implies a mechanistic link between these 2 signaling pathways.

Extrapolating this to the in vivo paradigm, there was a concomitant increase in Sgk1 and NPR-A gene expression in the renal medulla of the intact rat and mouse that was accompanied by increased urinary cGMP and sodium excretion following only 24 hours of water restriction. Dehydration of Npr1–/– mice elevated urinary osmolality and Sgk1 expression in the renal medulla but failed to elicit changes in urinary cGMP or sodium excretion. We believe that this supports our hypothesis that the liganded NPR-A in the distal nephron is a critical contributor to dehydration-induced natriuresis.

While we have carried out the majority of our studies using IMCD, it is conceivable, if not probable, that other distal nephron segments (e.g., outer medullary or cortical collecting duct) participate in generating the natriuresis. In fact, we have examined the osmotic response to water restriction in rat renal outer medullary tissue and found a similar increase in Sgk1 and NPR-A expression, though the increases were smaller than those seen for IMCD (S. Chen, unpublished observations).

Recent work by Rubera et al. (58) demonstrated that targeted deletion of the gene encoding the αENaC from the collecting duct of the mouse had no major effect on sodium homeostasis. We interpret this finding to mean that ENaC activity in the collecting duct is dispensable with regard to the maintenance of sodium balance at steady state. It could reflect the fact that the collecting duct system plays no role in maintenance of sodium homeostasis under the conditions examined. Alternatively, it could mean that loss of collecting duct activity can be accommodated, perhaps through developmental compensation, by residual transport activity in more proximal nephron segments. It is also possible that extinction of ENaC activity in the collecting duct was less than complete, a possibility acknowledged by the authors (58). In any case, sodium reabsorption that is inhibitable by ANP has been demonstrated in IMCD (59). Whether this ANP-dependent natriuresis results from inhibition of ENaC activity (60) as opposed to increased paracellular permeability with backflux of sodium into the tubular fluid, as suggested previously (61), remains to be determined.

It is equally noteworthy that expression of the ANP gene in renal collecting duct is also increased in this setting. The combination of increased NPR-A expression and increased ligand availability would be expected to significantly increase urinary sodium excretion. This natriuresis occurs under conditions where renal ANP gene regulation is in direct opposition to that of its atrial counterpart, implying that a totally independent regulatory circuitry governs its expression. The details of this regulatory circuitry remain undefined. It does not appear to be osmoregulatory, since hypertonicity does not increase ANP gene expression in isolated cortical or medullary collecting duct cells (data not shown).

Collectively, these studies and those of others (111) indicate that physiological systems, independent of those that control water intake and retention, are in place to protect the upper border of serum sodium concentration. Under conditions where intravascular volume is largely preserved, these systems are capable of promoting an increase in urinary sodium excretion. We believe that this occurs, at least in part, through activation of the natriuretic peptide–dependent signaling system in the distal nephron, an effect that requires the osmotic stimulation of Sgk1 gene expression. This renal natriuretic peptide system would be predicted to play an important role in dampening swings in serum sodium concentration attendant to transient periods of water deprivation. One might also envision that aberrant activation of this system could contribute to the paradoxical increase in renal sodium wasting seen in the syndrome of inappropriate antidiuretic hormone secretion (62, 63) or cerebral salt wasting syndrome (62).


Plasmid construction and mutagenesis.

A 1,430-bp segment of 5′ flanking sequence from the rat Sgk1-CAT reporter provided by Gary Firestone (University of California Berkeley, Berkeley, California, USA) was amplified and subcloned into pGL3 using newly generated KpnI and BglII restriction sites at opposing ends of the fragment. The structure was confirmed by DNA sequencing. Mutagenesis of the putative TonE (–335 GGGAGAGGAAATGGAAATCACCGAGGCTCTCC; TonE underlined) was carried out using the QuikChange Mutagenesis Kit (Stratagene) and the following series of oligonucleotides (sequence represents sense strand, with mutagenized bases represented in lower case): M1 (–335 GGGAGAGGAAATaGAAAATCACCGAGGCTCTCC), M2 (–335 GGGAGAGGAAATGGgAAATCACCGAGGCTCTCC), M3 (–335 GGGAGAGGAAATaaAAAATCAtCGAGGCTCTCC), and M4 (–335 GGGAGAGGAAATGGAAAATCACtGAGGCTCTCC). A GC-rich region spanning an Sp1-binding site was identified in the Sgk1 gene promoter previously (34) (–67 CCTGGTCCCGCCTGCCCCGCCCCCTGGAGGCTC; Sp1-binding site underlined). An Sp1 mutant (–67 CCTGGTCCCGCCTGCCttGCaaCCTGGAGGCTC) was created in this promoter using base modifications identical to those reported previously (34). The M3/Sp1 mutant (–335 GGGAGAGGAAATaaAAAATCAtCGAGGCTCTCC/–67 CCTGGTCCCGCCTGCCttGCaaCCTGGAGGCTC) was generated using combined mutagenesis of the promoter.

Primary cultures of rat IMCD cells.

All experiments in animals were reviewed and approved by the IACUC of UCSF. Adult Sprague-Dawley rats were euthanized by CO2 narcosis, followed by bilateral thoracotomy. The inner medullary tissue of each kidney was dissected, minced, and digested with 1 mg/ml collagenase at 37°C, with gentle agitation during each 30-minute cycle. The preparation was enriched for IMCD cells using hypotonic lysis as described previously (64). Cells were resuspended in medium-1 (65) and seeded onto culture plates. After 18–24 hours, the medium was changed to K-1 medium (65) prior to initiation of the experiment.

Preparation of nuclear extracts.

IMCD cells were cultured and treated with vehicle or NaCl for 4–5 hours. Cells were harvested and lysed with buffer A (10 mM HEPES, pH 7.9, 1.5 mM MgCl2, 10 mM KCl, 0.5% Nonidet P-40, 1 mM dithiothreitol, protease inhibitor cocktail [1 Complete tablet/50 ml; Roche]) on ice for 10 minutes. Lysates were centrifuged for 5 minutes at 4°C. Supernatants were transferred to new tubes and adjusted to 150 mM NaCl and 10% glycerol prior to Western blot analysis for cytoplasmic NFAT5. Particulates were resuspended in buffer C (20 mM HEPES, pH 7.9, 420 mM NaCl, 1.5 mM MgCl2, 0.2 mM EDTA, 25% glycerol, and the protease inhibitor cocktail) and kept on ice for 30 minutes. Nuclear suspensions were centrifuged at 12,800 g for 10 minutes, and the nuclear extracts were stored at –80°C for later EMSA or immunoblotting.


Oligonucleotides used for EMSAs were as follows: wild-type: (–335 GGGAGAGGAAATGGAAAATCACCGAGGCTCTCC); M1 (–335 GGGAGAGGAAATaGAAAATCACCGAGGCTCTCC); M2 (–335 GGGAGAGGAAATGGgAAATCACCGAGGCTCTCC); M3 (–335 GGGAGAGGAAATaaAAAATCAtCGAGGCTCTCC); M4 (–335 GGGAGAGGAAATGGAAAATCACtGAGGCTCTCC). The oligonucleotides containing the wild-type or mutant (lower-case lettering) OREs (underlined) were annealed with their complementary primer sequence and purified using a QIAquick Nucleotide Removal Kit (QIAGEN). Nuclear extracts (5 μg) were incubated in binding reaction buffer [10 mM HEPES, pH 7.9, 50 mM KCl, 0.2 mM EDTA, 2.5 mM dithiothreitol, 10% glycerol, and 0.05% Nonidet P-40, containing 1 μg of poly(dI-dC)] and 32P-end-labeled double-stranded wild-type oligonucleotide at room temperature for 30 minutes. For immunoperturbation experiments, nuclear extracts were preincubated on ice for 2 hours with 1 μg of polyclonal antibody directed against NFAT5 (Affinity BioReagents) or the p50 subunit of NF-κB (Santa Cruz Biotechnology Inc.). NFAT5 antibody used in pilot experiments was provided by H. Moo Kwon (University of Maryland School of Medicine, Baltimore, Maryland, USA). All samples were resolved on 4% nondenaturing polyacrylamide gels. Gels were dried and exposed to X-ray film.

Transfection and luciferase assay.

IMCD cells were cultured as described above and then transiently transfected with 1 μg of –1,430 rat Sgk1-luciferase (wild-type or mutant) and 0.2 μg of actin–β-galactosidase, in the presence or absence of U6 shRNA-NFAT5 (U6-N5 ex8) or a scrambled shRNA as a negative control (U6-N) (46) or NFAT5-DN (46), a dominant negative mutant of NFAT5, using Lipofectin Reagent (Invitrogen) under conditions recommended by the manufacturer. U6 shRNA-NFAT5 and NFAT5-DN were gifts from Anne Goldfeld (Harvard Medical School, Boston, Massachusetts, USA). Twenty four hours after transfection, cells were treated with 75 mM NaCl or 150 mM sucrose in DMEM (296 mOsm/kg H2O) for 24 hours, after which cells were washed twice with PBS and lysed with passive lysis buffer (Promega). Luciferase activity was measured using the Luciferase Assay System (Promega). β-Galactosidase activity was assayed using the Galacto-Light Plus chemiluminescence assay (Tropix, Applied Biosystems). Luciferase levels in individual samples were normalized to β-galactosidase activity.

ChIP assay.

Two 15-cm plates of approximately 80% confluent rat IMCD cells were cultured for 24 hours. NaCl (75 mM) or sucrose (150 mM) treatment in DMEM culture medium was performed for 4 hours. Cells (two 15-cm plates per experimental condition) were then crosslinked with 1% formaldehyde (final concentration) for 10 minutes at room temperature. The reaction was stopped by addition of glycine to a final concentration of 0.125 M for 5 minutes at room temperature. Cells were washed with cold PBS and scraped into 50-ml tubes. Cells were lysed in 10 ml cell lysis buffer (5 mM PIPES, pH 8.0, 85 mM KCl, 0.5% NP-40, and protease inhibitor cocktail) for 10 minutes on ice. Released nuclei were lysed in 2 ml nuclear lysis buffer (50 mM Tris-HCl, pH 8.1, 10 mM EDTA, 1% SDS, and protease inhibitor cocktail) for another 10 minutes on ice. Nuclear lysates were sonicated to a final average fragment length of 1 kb. Sonicated chromatin was cleared by centrifugation at 20,800 g 4°C for 10 minutes. Two hundred micrograms of sheared chromatin was used for each immunoprecipitation. Chromatin was first precleared with 100 μl BSA- and salmon sperm DNA–blocked Protein A Sepharose (GE Healthcare) beads for 1 hour at 4°C. Two micrograms of normal rabbit serum or specific antibody (see Figure Figure5)5) was added to each 100 μg of precleared chromatin and incubated overnight on a rotating platform at 4°C. The following morning, another 100 μl of beads was added to collect precipitated complexes. Beads were sequentially washed in 4 different buffers: TSE I buffer (0.1% SDS, 1% Triton X-100, 2 mM EDTA, 20 mM Tris-HCl, pH 8.1, 150 mM NaCl), TSE II buffer (same as TSE I with addition of 500 mM NaCl), ChIP buffer III (0.25 mM LiCl, 1% NP-40, 1% deoxycholate, 1 mM EDTA, 10 mM Tris-HCl, pH 8.1), and TE buffer (1 mM EDTA, 10 mM Tris-HCl, pH 8.1). Precipitated complexes were eluted twice from the beads in fresh elution buffer (1% SDS, 0.1 M NaHCO3) for 30 minutes each at room temperature. Crosslinking was reversed overnight at 65–67°C. The next morning, samples were precipitated with NaCl and ethanol (100%). Pellets were resuspended in 100 μl TE buffer. Two microliters of high-concentration RNase A (1579681; Roche) was added, and the sample was incubated for 2 hours at 37°C. At that point, 25 μl 5× PK buffer (50 mM Tris-HCl, pH 7.5, 25 mM EDTA, 1.25% SDS, and 1.5 μl proteinase K [25 mg/ml]) was added, and the incubation was continued another 2 hours at 55°C. Samples were extracted with phenol:chloroform:isoamylalcohol, followed by chloroform:isoamylalcohol. DNA was precipitated and quantified by NanoDrop (Thermo Scientific). Ten nanograms of precipitated DNA were used per PCR reaction. Primer locations are shown in Figure Figure5;5; their sequences are provided below. PCR was carried out under standard conditions with annealing temperature of 58°C for 32 cycles.

To study the interaction of protein binding with exogenous (i.e., transiently transfected) rat Sgk1 gene promoter sequence, IMCD cells were transfected with 20 μg –1,430 Sgk1-Luc or –1,430 M3-Sgk1-Luc, cultured for 44 hours, and treated with sucrose (150 mM) or NaCl (75 mM) in DMEM for 4 hours prior to collection, chromatin preparation, and analysis (as described above).

Four primers were used to amplify TonE and non-TonE-containing fragments in the endogenous rat Sgk1 promoter (primer 1: 5′-GAGATCAGGGCGGAGTACAG-3′, primer 2: 5′-AGAACCGAGGCTTCCACAG-3′, primer 3: 5′-ACCGTCATCTTTCAGCGTTT-3′, primer 4: 5′-TTGCCCTGGAGCTTTAATGT-3′) (see Figure Figure55 for the position of these primers). The TonE fragment in the transfected Sgk1 promoter sequence was obtained by using primers 1 and 5 (see Figure Figure5).5). The latter is an antisense primer in the luciferase gene coding sequence (primer 5: 5′-CTTCCAGCGGATAGAATGGC-3′).

In vivo dehydration studies.

Adult male Sprague-Dawley rats, weighing approximately 250 g, were used in this study. Before water restriction, the rats were weighed and transferred to clean metabolic cages. A control group of animals had free access to water and standard chow. The 24-hour water-restricted group was provided only with chow. Urine was collected during the last 15 hours. An aliquot from the final 15-hour urine sample was used to measure osmolality and sodium. On completion of 24-hour water deprivation, animals were anesthetized by intraperitoneal injection of Inactin (Sigma-Aldrich) (100 mg/kg) and weighed. Blood pressure was measured by insertion of a tapered polyethylene catheter into the carotid artery. The catheter was connected to a Statham blood pressure transducer attached to a direct writing recorder. Blood was collected in ice-cold tubes containing Na2EDTA and aprotinin. Plasma was prepared for immediate measurement of osmolality and sodium and stored at –70°C for later measurements of aldosterone using an EIA kit (Cayman Chemical) and ANP using an ANP RIA kit (Phoenix Pharmaceuticals Inc.). Urine was collected for the final 2 hours for measurement of volume, sodium, cyclic GMP (cyclic GMP RIA kit; PerkinElmer), and immunoreactive urodilatin (urodilatin RIA kit; Phoenix Pharmaceuticals Inc.). More than 99% of natriuretic peptide immunoreactivity in the urine reflects urodilatin (66). The inner medullas of paired kidneys were isolated for the measurements of Sgk1, NPR-A, urodilatin, αENaC, β-tubulin, and GAPDH mRNAs and/or proteins. Urine and plasma sodium were measured by flame photometry (model 943; Instrumentation Laboratory). Urine and plasma osmolalities were determined by osmometry (Advanced Instruments).

Npr1–/– mice were purchased from The Jackson Laboratory (stock 004374).

Mouse blood pressure was measured using the tail-cuff method. Mice were trained on the Hatteras Instruments SC1000 Blood Pressure Analysis System according to manufacturer’s instructions for 4 days. Ten consecutive measurements on the last day were averaged to calculate systolic and diastolic blood pressure. Adult wild-type and Npr1–/– mice were subjected to 24-hour water deprivation, while their respective control mice had free access to water. Urine was collected during the last 15 hours. An aliquot from the final 15-hour urine sample was used to measure osmolality, sodium, and cGMP concentration. Renal inner medullas were isolated for measurement of NPR-A and Sgk1 protein expression.

RNA isolation and real-time PCR analysis.

Total RNA from isolated renal inner medullas, atria, and IMCD cells were prepared using the RNeasy Mini Kit (QIAGEN). Six hundred nanograms of total RNA were reverse transcribed into cDNA using Superscript III reverse transcriptase (Invitrogen). Real-time PCR was performed with rat ANP (catalog Rn00561661_ml) and GAPDH (catalog Rn99999916_sl) Taqman primers (Applied Biosystems) and rat Sgk1 (sense: CAAGGAGAACATCGAGCACA; antisense: TTTCAGCTGGAGAGGCTTGT), NPR-A (sense: GGAGAAGCCCTCAAGATCCACT; antisense: CTTGCCTTTGCCCTTCATTTC), and GAPDH (sense: GACATGCCGCCTGGAGAAAC; antisense: AGCCCAGGATGCCCTTTAGT) SYBR Green (Applied Biosystems) primers. ANP, sgk1, and NPR-A transcript levels were quantified and normalized to GAPDH transcript levels in each sample. The thermal cycles of the ABI Prism 7900 Sequence Detection System (Applied Biosystems) were 50°C for 2 minutes, 95°C for 10 minutes, for Taqman activation, followed by 40 cycles of 95°C for 15 seconds and 60°C for 60 seconds.


The isolated renal inner medulla from rats and mice was immediately homogenized in lysis buffer (50 mM Tris-HCl, pH 7.5; 150 mM NaCl, 1% Triton X-100, 5 mM EDTA, 10% glycerol, 1 mM sodium orthovanadate, 10 mM sodium fluoride, 1 mM glycerophosphate) containing protease inhibitors (1 Complete tablet/50 ml). For cultured IMCD cells, cells were collected, pelleted, and then lysed with the same lysis buffer. Forty micrograms of total protein was denatured at 100°C for 5 minutes, subjected to 9% SDS-PAGE, and transferred onto Immun-Blot PVDF membranes (Bio-Rad). Membranes were blocked with 5% nonfat milk in TBST (50 mM Tris-HCl, pH 7.5; 150 mM NaCl, 0.1% Tween-20) and probed with a mouse monoclonal antibody directed against Sgk1 (sc-28338; Santa Cruz Biotechnology Inc.) or a goat polyclonal IgG directed against αENaC (sc-22239; Santa Cruz Biotechnology Inc.). An HRP-conjugated secondary antibody was used to detect immunoreactive bands using the ECL Western blotting detection system (Amersham, GE Healthcare). The same membranes were reblotted with anti-GAPDH antibody (sc-32233; Santa Cruz Biotechnology Inc.). Sgk1 and αENaC signals were quantified using a Kodak Scientific Imaging system and normalized to the GAPDH signal.

For preparation of the membrane fraction, IMCD cells were treated with 75 mM NaCl for 24 hours and then scraped into ice-cold PBS. After brief centrifugation, cells were resuspended in buffer A (20 mM Tris, pH 7.5, 10 mM mannitol, and protease inhibitors) and homogenized. Isolated renal inner medullary tissue from rats or mice was homogenized in buffer A as described above. After centrifugation at 800 g for 10 minutes, soluble and membrane fractions from either cultured cells or medullary tissue were separated by centrifugation at 150,000 g for 1 hour at 4°C. The particulate fractions were resuspended in the lysis buffer described above containing 2% Triton X-100. Forty micrograms of membrane protein was heated at 37°C for 15 minutes for Western blotting and probed with NPR-A antibody (PGCA-101AP; FabGennix Inc.). Chemiluminescence detection of rat and mouse NPR-A employed ECL and SuperSignal West Femto (Pierce Protein Research Products, Thermo Scientific), respectively. The same membrane was washed and reprobed with β-tubulin antibody (sc-9104; Santa Cruz Biotechnology Inc.). NPR-A signal was quantified using a Kodak Scientific Imaging system and normalized to the β-tubulin signal.

siRNA silencing of Sgk1 and NPR-A genes.

Twenty-one nucleotide-annealed duplex siRNAs directed against rat Sgk1 gene sequence (siSgk1A, GGAGCCCGAACUUAUGAACtt; siSgk1B, CCAUCAUUUUAAUGUCCUGtt; and siSgk1C GGUUCUUCUAGCAAGGCACtt — all sense strand) were chemically synthesized and purified using a commercial source (Ambion, Applied Biosystems), as was a negative control siRNA (Ambion, Applied Biosystems) containing a 19-bp scrambled sequence. The latter sequences have no significant homology to any known gene sequences from the rat genome. IMCD cells were cultured to 60%–70% confluence and then transfected with 100 pmol siSgk1A, siSgk1B, siSgk1C, or the negative control siRNA using Oligofectamine (Invitrogen) according to the manufacturer’s instructions. Forty-eight hours after transfection, cells were washed, and cellular lysates were prepared and analyzed for Sgk1 and NPR-A mRNAs and proteins by real-time PCR and Western blot analysis.


Data were analyzed by 1-way ANOVA using the Newman-Keuls test to assess statistical differences between multiple groups. One-tailed Student’s t test was used for comparisons between 2 groups. All data are presented as mean ± SD. A P value less than 0.05 was considered statistically significant.


Antibody directed against NFAT5 for pilot experiments was generously provided by H. Moo Kwon. U6 ShRNAi-NFAT5 and NFAT5-DN were gifts from Anne Goldfeld. We are grateful for the rat Sgk1-CAT reporter provided by Gary Firestone. We are grateful to D. Pearce for critical reading of the manuscript and D. Glenn for technical advice on the ChIP analyses. This work was supported by NIH grants HL45637 (to D.G. Gardner) and HL68871 (to M.H. Humphreys).


Conflict of interest: The authors have declared that no conflict of interest exists.

Nonstandard abbreviations used: αENaC, α subunit of ENaC; ANP, atrial natriuretic peptide; ENaC, epithelial sodium channel; IMCD, inner medullary collecting duct; NFAT, nuclear factor of activated T cells; NPR-A, type A natriuretic peptide receptor; Sgk1, serum- and glucocorticoid-inducible kinase; TonE, tonicity-responsive enhancer; TonEBP, TonE-binding protein.

Citation for this article: J. Clin. Invest. 119:1647–1658 (2009). doi:10.1172/JCI35314


1. Andersen L.J., Andersen J.L., Pump B., Bie P. Natriuresis induced by mild hypernatremia in humans. Am. J. Physiol. Regul. Integr. Comp. Physiol. 2002;282:R1754–R1761. [PubMed]
2. Huang W., Lee S.L., Arnason S.S., Sjoquist M. Dehydration natriuresis in male rats is mediated by oxytocin. Am. J. Physiol. 1996;270:R427–R433. [PubMed]
3. Lucke C., Erbler H., Herting T., Dohler K.D. Secretion of arginin-vasopressin, aldosterone and corticosterone and plasma-renin activity in water-deprived rats. Contrib. Nephrol. 1980;19:63–70. [PubMed]
4. Luke R.G. Natriuresis and chloruresis during hydrogenia in the rat. Am. J. Physiol. 1973;224:13–20. [PubMed]
5. McKenna T.M., Haines H. Sodium metabolism during acclimation to water restriction by wild mice, Mus musculus. Am. J. Physiol. 1981;240:R319–R326. [PubMed]
6. McKinley M.J., Denton D.A., Nelson J.F., Weisinger R.S. Dehydration induces sodium depletion in rats, rabbits, and sheep. Am. J. Physiol. 1983;245:R287–R292. [PubMed]
7. McKinley M.J., Evered M.D., Mathai M.L. Renal Na excretion in dehydrated and rehydrated adrenalectomized sheep maintained with aldosterone. Am. J. Physiol. Regul. Integr. Comp. Physiol. 2000;279:R17–R24. [PubMed]
8. Merrill D.C., Skelton M.M., Cowley A.W., Jr. Humoral control of water and electrolyte excretion during water restriction. Kidney Int. 1986;29:1152–1161. doi: 10.1038/ki.1986.121. [PubMed] [Cross Ref]
9. Metzler G.H., Thrasher T.N., Keil L.C., Ramsay D.J. Endocrine mechanisms regulating sodium excretion during water deprivation in dogs. Am. J. Physiol. 1986;251:R560–R568. [PubMed]
10. Thrasher T.N., Wade C.E., Keil L.C., Ramsay D.J. Sodium balance and aldosterone during dehydration and rehydration in the dog. Am. J. Physiol. 1984;247:R76–R83. [PubMed]
11. Zucker A., Gleason S.D., Schneider E.G. Renal and endocrine response to water deprivation in dog. Am. J. Physiol. 1982;242:R296–R302. [PubMed]
12. Huang W., Lee S.L., Sjoquist M. Natriuretic role of endogenous oxytocin in male rats infused with hypertonic NaCl. Am. J. Physiol. 1995;268:R634–R640. [PubMed]
13. Ko B.C., Ruepp B., Bohren K.M., Gabbay K.H., Chung S.S. Identification and characterization of multiple osmotic response sequences in the human aldose reductase gene. J. Biol. Chem. 1997;272:16431–16437. doi: 10.1074/jbc.272.26.16431. [PubMed] [Cross Ref]
14. Miyakawa H., et al. Cis- and trans-acting factors regulating transcription of the BGT1 gene in response to hypertonicity. Am. J. Physiol. 1998;274:F753–F761. [PubMed]
15. Ito T., et al. Expression of taurine transporter is regulated through the TonE (tonicity-responsive element)/TonEBP (TonE-binding protein) pathway and contributes to cytoprotection in HepG2 cells. Biochem. J. 2004;382:177–182. doi: 10.1042/BJ20031838. [PMC free article] [PubMed] [Cross Ref]
16. Woo S.K., Lee S.D., Na K.Y., Park W.K., Kwon H.M. TonEBP/NFAT5 stimulates transcription of HSP70 in response to hypertonicity. Mol. Cell. Biol. 2002;22:5753–5760. doi: 10.1128/MCB.22.16.5753-5760.2002. [PMC free article] [PubMed] [Cross Ref]
17. Rim J.S., et al. Transcription of the sodium/myo-inositol cotransporter gene is regulated by multiple tonicity-responsive enhancers spread over 50 kilobase pairs in the 5′-flanking region. J. Biol. Chem. 1998;273:20615–20621. doi: 10.1074/jbc.273.32.20615. [PMC free article] [PubMed] [Cross Ref]
18. Nakayama Y., Peng T., Sands J.M., Bagnasco S.M. The TonE/TonEBP pathway mediates tonicity-responsive regulation of UT-A urea transporter expression. J. Biol. Chem. 2000;275:38275–38280. doi: 10.1074/jbc.M004678200. [PubMed] [Cross Ref]
19. Hasler U., et al. Tonicity-responsive enhancer binding protein is an essential regulator of aquaporin-2 expression in renal collecting duct principal cells. J. Am. Soc. Nephrol. 2006;17:1521–1531. doi: 10.1681/ASN.2005121317. [PubMed] [Cross Ref]
20. Miyakawa H., Woo S.K., Dahl S.C., Handler J.S., Kwon H.M. Tonicity-responsive enhancer binding protein, a rel-like protein that stimulates transcription in response to hypertonicity. Proc. Natl. Acad. Sci. U. S. A. 1999;96:2538–2542. doi: 10.1073/pnas.96.5.2538. [PMC free article] [PubMed] [Cross Ref]
21. Stroud J.C., Lopez-Rodriguez C., Rao A., Chen L. Structure of a TonEBP-DNA complex reveals DNA encircled by a transcription factor. Nat. Struct. Biol. 2002;9:90–94. doi: 10.1038/nsb749. [PubMed] [Cross Ref]
22. Lee S.D., Woo S.K., Kwon H.M. Dimerization is required for phosphorylation and DNA binding of TonEBP/NFAT5. Biochem. Biophys. Res. Commun. 2002;294:968–975. doi: 10.1016/S0006-291X(02)00572-7. [PubMed] [Cross Ref]
23. Lopez-Rodriguez C., Aramburu J., Rakeman A.S., Rao A. NFAT5, a constitutively nuclear NFAT protein that does not cooperate with Fos and Jun. Proc. Natl. Acad. Sci. U. S. A. 1999;96:7214–7219. doi: 10.1073/pnas.96.13.7214. [PMC free article] [PubMed] [Cross Ref]
24. Dahl S.C., Handler J.S., Kwon H.M. Hypertonicity-induced phosphorylation and nuclear localization of the transcription factor TonEBP. Am. J. Physiol. Cell Physiol. 2001;280:C248–C253. [PubMed]
25. Zhang Z., et al. Ataxia telangiectasia-mutated, a DNA damage-inducible kinase, contributes to high NaCl-induced nuclear localization of transcription factor TonEBP/OREBP. Am. J. Physiol. Renal Physiol. 2005;289:F506–F511. doi: 10.1152/ajprenal.00417.2004. [PubMed] [Cross Ref]
26. Cha J.H., et al. Hydration status affects nuclear distribution of transcription factor tonicity responsive enhancer binding protein in rat kidney. J. Am. Soc. Nephrol. 2001;12:2221–2230. [PubMed]
27. Cai Q., Ferraris J.D., Burg M.B. High NaCl increases TonEBP/OREBP mRNA and protein by stabilizing its mRNA. Am. J. Physiol. Renal Physiol. 2005;289:F803–F807. doi: 10.1152/ajprenal.00448.2004. [PubMed] [Cross Ref]
28. Woo S.K., Dahl S.C., Handler J.S., Kwon H.M. Bidirectional regulation of tonicity-responsive enhancer binding protein in response to changes in tonicity. Am. J. Physiol. Renal Physiol. 2000;278:F1006–F1012. [PubMed]
29. Webster M.K., Goya L., Ge Y., Maiyar A.C., Firestone G.L. Characterization of sgk, a novel member of the serine/threonine protein kinase gene family which is transcriptionally induced by glucocorticoids and serum. Mol. Cell. Biol. 1993;13:2031–2040. [PMC free article] [PubMed]
30. Leong M.L., Maiyar A.C., Kim B., O’Keeffe B.A., Firestone G.L. Expression of the serum- and glucocorticoid-inducible protein kinase, Sgk, is a cell survival response to multiple types of environmental stress stimuli in mammary epithelial cells. J. Biol. Chem. 2003;278:5871–5882. doi: 10.1074/jbc.M211649200. [PubMed] [Cross Ref]
31. Lang F., et al. Deranged transcriptional regulation of cell-volume-sensitive kinase hSGK in diabetic nephropathy. Proc. Natl. Acad. Sci. U. S. A. 2000;97:8157–8162. doi: 10.1073/pnas.97.14.8157. [PMC free article] [PubMed] [Cross Ref]
32. Waldegger S., et al. h-sgk serine-threonine protein kinase gene as transcriptional target of transforming growth factor beta in human intestine. Gastroenterology. 1999;116:1081–1088. doi: 10.1016/S0016-5085(99)70011-9. [PubMed] [Cross Ref]
33. Chen S.Y., et al. Epithelial sodium channel regulated by aldosterone-induced protein sgk. Proc. Natl. Acad. Sci. U. S. A. 1999;96:2514–2519. doi: 10.1073/pnas.96.5.2514. [PMC free article] [PubMed] [Cross Ref]
34. Bell L.M., et al. Hyperosmotic stress stimulates promoter activity and regulates cellular utilization of the serum- and glucocorticoid-inducible protein kinase (Sgk) by a p38 MAPK-dependent pathway. J. Biol. Chem. 2000;275:25262–25272. doi: 10.1074/jbc.M002076200. [PubMed] [Cross Ref]
35. Klingel K., et al. Expression of cell volume-regulated kinase h-sgk in pancreatic tissue. Am. J. Physiol. Gastrointest. Liver Physiol. 2000;279:G998–G1002. [PubMed]
36. Waldegger S., Barth P., Forrest J.N., Jr., Greger R., Lang F. Cloning of sgk serine-threonine protein kinase from shark rectal gland - a gene induced by hypertonicity and secretagogues. Pflugers Arch. 1998;436:575–580. doi: 10.1007/s004240050674. [PubMed] [Cross Ref]
37. Waldegger S., Barth P., Raber G., Lang F. Cloning and characterization of a putative human serine/threonine protein kinase transcriptionally modified during anisotonic and isotonic alterations of cell volume. Proc. Natl. Acad. Sci. U. S. A. 1997;94:4440–4445. doi: 10.1073/pnas.94.9.4440. [PMC free article] [PubMed] [Cross Ref]
38. Waldegger S., Gabrysch S., Barth P., Fillon S., Lang F. h-sgk serine-threonine protein kinase as transcriptional target of p38/MAP kinase pathway in HepG2 human hepatoma cells. Cell. Physiol. Biochem. 2000;10:203–208. doi: 10.1159/000016351. [PubMed] [Cross Ref]
39. Uawithya P., Pisitkun T., Ruttenberg B.E., Knepper M.A. Transcriptional profiling of native inner medullary collecting duct cells from rat kidney. Physiol. Genomics. 2008;32:229–253. [PMC free article] [PubMed]
40. Chen S., et al. Sgk1 mediates osmotic induction of NPR-A gene in rat inner medullary collecting duct cells. Hypertension. 2004;43:866–871. doi: 10.1161/01.HYP.0000121883.55722.45. [PubMed] [Cross Ref]
41. Chen S., Gardner D.G. Osmoregulation of natriuretic peptide receptor signaling in inner medullary collecting duct. A requirement for p38 MAPK. J. Biol. Chem. 2002;277:6037–6043. doi: 10.1074/jbc.M111117200. [PubMed] [Cross Ref]
42. Cowley B.D., Jr., Ferraris J.D., Carper D., Burg M.B. In vivo osmoregulation of aldose reductase mRNA, protein, and sorbitol in renal medulla. Am. J. Physiol. 1990;258:F154–F161. [PubMed]
43. Yamauchi A., et al. In vivo osmoregulation of Na/myo-inositol cotransporter mRNA in rat kidney medulla. J. Am. Soc. Nephrol. 1994;5:62–67. [PubMed]
44. Ferraris J.D., Williams C.K., Ohtaka A., Garcia-Perez A. Functional consensus for mammalian osmotic response elements. Am. J. Physiol. 1999;276:C667–C673. [PubMed]
45. Daoudal S., Tournaire C., Halere A., Veyssiere G., Jean C. Isolation of the mouse aldose reductase promoter and identification of a tonicity-responsive element. J. Biol. Chem. 1997;272:2615–2619. doi: 10.1074/jbc.272.5.2615. [PubMed] [Cross Ref]
46. Esensten J.H., et al. NFAT5 binds to the TNF promoter distinctly from NFATp, c, 3 and 4, and activates TNF transcription during hypertonic stress alone. Nucleic Acids Res. 2005;33:3845–3854. doi: 10.1093/nar/gki701. [PMC free article] [PubMed] [Cross Ref]
47. Rozansky D.J., et al. Hypotonic induction of SGK1 and Na+ transport in A6 cells. Am. J. Physiol. Renal Physiol. 2002;283:F105–F113. [PubMed]
48. Hills C.E., Bland R., Bennett J., Ronco P.M., Squires P.E. High glucose up-regulates ENaC and SGK1 expression in HCD-cells. Cell. Physiol. Biochem. 2006;18:337–346. doi: 10.1159/000097611. [PubMed] [Cross Ref]
49. Vasquez M.M., et al. Induction of serum- and glucocorticoid-induced kinase-1 (SGK1) by cAMP regulates increases in alpha-ENaC. J. Cell. Physiol. 2008;217:632–642. doi: 10.1002/jcp.21534. [PubMed] [Cross Ref]
50. Forssmann W.G., Richter R., Meyer M. The endocrine heart and natriuretic peptides: histochemistry, cell biology, and functional aspects of the renal urodilatin system. Histochem. Cell Biol. 1998;110:335–357. doi: 10.1007/s004180050295. [PubMed] [Cross Ref]
51. Schulz-Knappe P., et al. Isolation and structural analysis of “urodilatin”, a new peptide of the cardiodilatin-(ANP)-family, extracted from human urine. Klin. Wochenschr. 1988;66:752–759. doi: 10.1007/BF01726570. [PubMed] [Cross Ref]
52. Forssmann W., Meyer M., Forssmann K. The renal urodilatin system: clinical implications. Cardiovasc. Res. 2001;51:450–462. doi: 10.1016/S0008-6363(01)00331-5. [PubMed] [Cross Ref]
53. Lopez M.J., et al. Salt-resistant hypertension in mice lacking the guanylyl cyclase-A receptor for atrial natriuretic peptide. Nature. 1995;378:65–68. doi: 10.1038/378065a0. [PubMed] [Cross Ref]
54. Tong E.H., et al. Regulation of nucleocytoplasmic trafficking of transcription factor OREBP/TonEBP/NFAT5. J. Biol. Chem. 2006;281:23870–23879. doi: 10.1074/jbc.M602556200. [PubMed] [Cross Ref]
55. Burg M.B., Kwon E.D., Kultz D. Regulation of gene expression by hypertonicity. Annu. Rev. Physiol. 1997;59:437–455. doi: 10.1146/annurev.physiol.59.1.437. [PubMed] [Cross Ref]
56. Jeon U.S., Kim J.A., Sheen M.R., Kwon H.M. How tonicity regulates genes: story of TonEBP transcriptional activator. Acta Physiol. (Oxf.). 2006;187:241–247. [PubMed]
57. Rasmussen M.S., Simonsen J.A., Sandgaard N.C., Hoilund-Carlsen P.F., Bie P. Effects of oxytocin in normal man during low and high sodium diets. Acta Physiol. Scand. 2004;181:247–257. doi: 10.1111/j.1365-201X.2004.01286.x. [PubMed] [Cross Ref]
58. Rubera I., et al. Collecting duct-specific gene inactivation of αENaC in the mouse kidney does not impair sodium and potassium balance. . J. Clin. Invest. 2003;112:554–565. [PMC free article] [PubMed]
59. Sonnenberg H., Honrath U., Wilson D.R. In vivo microperfusion of inner medullary collecting duct in rats: effect of amiloride and ANF. Am. J. Physiol. 1990;259:F222–F226. [PubMed]
60. Light D.B., Schwiebert E.M., Karlson K.H., Stanton B.A. Atrial natriuretic peptide inhibits a cation channel in renal inner medullary collecting duct cells. Science. 1989;243:383–385. doi: 10.1126/science.2463673. [PubMed] [Cross Ref]
61. Sonnenberg H., Honrath U., Chong C.K., Wilson D.R. Atrial natriuretic factor inhibits sodium transport in medullary collecting duct. Am. J. Physiol. 1986;250:F963–F966. [PubMed]
62. Palmer B.F. Hyponatremia in patients with central nervous system disease: SIADH versus CSW. Trends Endocrinol. Metab. 2003;14:182–187. doi: 10.1016/S1043-2760(03)00048-1. [PubMed] [Cross Ref]
63. Baylis P.H. The syndrome of inappropriate antidiuretic hormone secretion. Int. J. Biochem. Cell Biol. 2003;35:1495–1499. doi: 10.1016/S1357-2725(03)00139-0. [PubMed] [Cross Ref]
64. Grenier F.C., Rollins T.E., Smith W.L. Kinin-induced prostaglandin synthesis by renal papillary collecting tubule cells in culture. Am. J. Physiol. 1981;241:F94–F104. [PubMed]
65. Chen S., Cao L., Intengan H.D., Humphreys M., Gardner D.G. Osmoregulation of endothelial nitric-oxide synthase gene expression in inner medullary collecting duct cells. Role in activation of the type A natriuretic peptide receptor. J. Biol. Chem. 2002;277:32498–32504. doi: 10.1074/jbc.M202321200. [PubMed] [Cross Ref]
66. Lee Y.J., Shin S.J., Tan M.S., Hsieh T.J., Tsai J.H. Increased renal atrial natriuretic peptide synthesis in rats with deoxycorticosterone acetate-salt treatment. Am. J. Physiol. 1996;271:F779–F789. [PubMed]

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