Correction
16 Mar 2009: Danielyan L, Zellmer S, Sickinger S, Tolstonog GV, Salvetter J, et al. (2009) Correction: Keratinocytes as Depository of Ammonium-Inducible Glutamine Synthetase: Age- and Anatomy-Dependent Distribution in Human and Rat Skin. PLOS ONE 4(3): 10.1371/annotation/fa1fbbb8-5dca-4afb-a5ee-c7eb3f5c45bc. https://doi.org/10.1371/annotation/fa1fbbb8-5dca-4afb-a5ee-c7eb3f5c45bc View correction
Figures
Abstract
In inner organs, glutamine contributes to proliferation, detoxification and establishment of a mechanical barrier, i.e., functions essential for skin, as well. However, the age-dependent and regional peculiarities of distribution of glutamine synthetase (GS), an enzyme responsible for generation of glutamine, and factors regulating its enzymatic activity in mammalian skin remain undisclosed. To explore this, GS localization was investigated using immunohistochemistry and double-labeling of young and adult human and rat skin sections as well as skin cells in culture. In human and rat skin GS was almost completely co-localized with astrocyte-specific proteins (e.g. GFAP). While GS staining was pronounced in all layers of the epidermis of young human skin, staining was reduced and more differentiated among different layers with age. In stratum basale and in stratum spinosum GS was co-localized with the adherens junction component ß-catenin. Inhibition of, glycogen synthase kinase 3β in cultured keratinocytes and HaCaT cells, however, did not support a direct role of ß-catenin in regulation of GS. Enzymatic and reverse transcriptase polymerase chain reaction studies revealed an unusual mode of regulation of this enzyme in keratinocytes, i.e., GS activity, but not expression, was enhanced about 8–10 fold when the cells were exposed to ammonium ions. Prominent posttranscriptional up-regulation of GS activity in keratinocytes by ammonium ions in conjunction with widespread distribution of GS immunoreactivity throughout the epidermis allows considering the skin as a large reservoir of latent GS. Such a depository of glutamine-generating enzyme seems essential for continuous renewal of epidermal permeability barrier and during pathological processes accompanied by hyperammonemia.
Citation: Danielyan L, Zellmer S, Sickinger S, Tolstonog GV, Salvetter J, Lourhmati A, et al. (2009) Keratinocytes as Depository of Ammonium-Inducible Glutamine Synthetase: Age- and Anatomy-Dependent Distribution in Human and Rat Skin. PLoS ONE 4(2): e4416. https://doi.org/10.1371/journal.pone.0004416
Editor: Christophe Egles, Tufts University, United States of America
Received: August 5, 2008; Accepted: December 23, 2008; Published: February 10, 2009
Copyright: © 2009 Danielyan et al. This is an open-access article distributed under the terms of the Creative Commons Attribution License, which permits unrestricted use, distribution, and reproduction in any medium, provided the original author and source are credited.
Funding: This study was supported by the Medical Faculties of the University of Tuebingen and Leipzig. The funders had no role in study design, data collection and analysis, decision to publish, or preparation of the manuscript.
Competing interests: Because of professional competition we would not trust the reviewing of this MS to the following scientists: 1. Häberle J, Klinik und Poliklinik für Kinder- und Jugendmedizin, Universitätsklinikum Münster, Albert-Schweitzer-Str. 33, 48129, Münster, Germany. 2. Häussinger D. Clinic for Gastroenterology, Hepatology and Infectiology, Heinrich-Heine-University Düsseldorf, Düsseldorf, Germany. 3. As well as any scientists from the above mentioned institutes.
Introduction
Glutamine synthetase (GS; EC 6.3.1.2) is the only known human enzyme capable of catalyzing glutamine (Gln) synthesis from ammonia and glutamate and, thereby, contributes to multiple tissue events regulated by this amino acid. Gln represents the most abundant amino acid in mammalian blood reflecting its function as the major shuttle of amino-nitrogen between cells. It plays an important role in acid-base homeostasis and serves as a fuel source for many types of cells. In rapidly dividing cells GS is required as a precursor for the synthesis of multiple biologically active compounds including purines, pyrimidines, and aminosugars [1]. Last but not least, Gln is a major constituent of proteins particularly in skin.
GS is found in many, if not all organs [2]. However, in most of them, expression of GS is confined to specific cell populations only. Prominent examples for this are the pericentral hepatocytes in liver [3], [4] and certain cells lining the proximal convoluted tubules in kidney [2], [5], [6]. In addition, GS at a lower but highly adaptive level is expressed in almost every organ in glial fibrillary acidic protein (GFAP)-producing perivascular cells that play an important role in tissue homeostasis at the blood-tissue interface [7]. These cells comprise astrocytes located at the blood brain barrier [8], activated hepatic stellate cells (HSC) at the blood-tissue interface in liver [9], and Leydig cells of the testis [10]. In pathological conditions, on the other hand, GS may be expressed in cells that normally do not produce the enzyme, such as neurons in Alzheimers disease. [11], [12], [13]. Thus, the cellular expression of GS in each organ is highly specific and has to be characterized by immunocytochemistry or similar techniques, in order to draw conclusions on its precise role and function.
Compared to many other organs, GS activity in rat skin has been found to be rather moderate [14], [15]. Consequently, interest in GS in skin remained low for a long time and this organ was not even mentioned in a comprehensive survey on GS in murine organs [16]. Even less is known so far about the cellular distribution as well as the specific function of GS in this organ. However, recent observations on humans with inherited GS deficiency convincingly showed the importance of GS for skin-specific functions. The consequences of this metabolic disease were illustrated by severely disturbed epidermal development, rapid appearance of focal erythema and blistering of the integumentum resulting in early postnatal death [17], [18]. These findings concerning integrity, regeneration and molecular characteristics of human and rodent skin propose a previously unrecognized considerable demand for Gln in the developing skin and an important local function of GS in skin integrity. An increased need for Gln during skin regeneration was also suggested by the finding that major burn injury of skin leads to the induction of GS expression in specific tissues such as lung, muscle, kidney and liver [19]. Likewise, thermal injury of 33–35% of body surface area is accompanied by increased levels of Gln in muscle, skin and adipose tissue preparations [20]. These studies call for detailed investigation of distribution of GS in different cell types and structures of the skin as well as mechanisms involved in the regulation of GS levels in keratinocytes.
Multiple structural and functional peculiarities and specific anatomy of the skin, offered an interesting object for further examination of our hypothesis concerning commonness of mechanisms operating at the border of different environments and tissues, i.e., blood-tissue, blood-urine and air-tissue interfaces. The co-localization in skin cells of several astrocyte-specific antigens [21] considerably strengthen our viewpoint concerning the universality of mechanisms regulating the homeostasis in different organs. This raised the question of whether the peculiar ability of smooth muscle alpha-actin (SMAA) and GFAP-containing astrocytes and HSC to express GS in a dynamic fashion contributing to tissue homeostasis and protection [7], [9], [22]–[24] may be found as well in epidermal keratinocytes forming part of the tissue-air interface.
To learn more about the skin-specific functions of GS we have investigated in detail the distribution of GS in different cell types and structures in human and rat skin samples of different age. In accordance with studies demonstrating a dependency of the antigenic composition of skin cells on their anatomy and age [25], [26], the specific cellular expression and localization of GS in different skin samples of humans and rats showed some variation depending on the age of the donor and on the location from which the skin sample was taken. These variations, for which we provide some prominent examples for different parts of skin from children and adult humans as well as from newborn and adult rats, indicate a close association of the specific cellular localization of GS with different functional and structural features of skin. In order to emphasize this association and, at the same time, to illustrate possible exceptions, we performed co-localizations of GS with each of the marker proteins previously shown to characterize these functional and structural differences [21]. Furthermore, we aimed at elucidating basic mechanisms involved in the regulation of GS levels in skin keratinocytes. In the light of recent in vitro studies demonstrating the influence of Gln on establishment of adherens and tight junctions complexes [27]–[30] and of the novel role of wingless-type mouse mammary tumour virus integration site family member (Wnt)/β-catenin signaling in regulating GS expression in liver [31], a series of investigations has been performed to examine the relation between GS and β-catenin. Our results suggest multiple roles of GS in maintaining barrier structure and function of skin supported by novel specific regulatory features.
Results
Cellular localization of GS in skin
Distribution of GS and its co-localization with GFAP and SMAA in human skin slices.
Double labeling of sections of human foreskin with polyclonal antibodies (pAb) directed against GS (green, Figure 1A) and monoclonal antibodies (mAb) against bovine GFAP (red, Figure 1B) revealed almost complete co-localization of both proteins in all layers of the epidermis: stratum basale (magenta arrows throughout Figure 1), stratum spinosum, stratum granulosum and stratum corneum (blue arrows throughout Figure 1). Similar spatial distribution of GS and GFAP was illustrated by intense yellow staining of epidermis in merged micrographs (Figure 1C). In young foreskin, the stratum corneum is very thin. The reaction of GS was particularly strong in stratum granulosum and stratum corneum and slightly weaker in stratum basale and stratum spinosum. In the dermis of these skin samples (white arrows), GS was expressed weaker than in epidermis (cf. structures indicated by blue and white arrows in Figures 1A, C). Similar findings for GS were obtained also in older foreskin (not shown).
(A–D) Expression of GS (A) and GFAP (B) and merged micrograph of GS and GFAP (C) immune reaction in human foreskin sections. (D–F) Expression of GS (D) and SMAA (E) and merged micrograph of GS and SMAA immune reaction (F) in a human skin section. The line connecting the D–F clearly shows strong expression of SMAA (E) in stratum granulosum and its absence of stratum corneum. The latter is strongly stained for GS (D). GS and SMAA merge at the interface of stratum corneum boarder and stratum granulosum (F). Binding of specific antibodies was visualized with FITC-conjugated goat anti-rabbit IgG and Cy3-conjugated goat anti-mouse IgG. Blue arrows point to stratum corneum, magenta arrows to stratum basale white arrows to fibroblasts and yellow arrows to small and middle-sized vessels. Scale bar: A–D, H 200 μm; E–G 100 μm.
In skin sections double-labeled with antibodies against GS and anti-SMAA, occasionally enhancement of GS staining in the nuclear area of the keratinocytes located in inner layers of the epidermis could be seen (Figure 1D). In accordance with our recent study [21], SMAA (Figure 1E, red) was preferentially localized in the perinuclear and nuclear area of human foreskin keratinocytes resulting in yellow or orange staining of this area in merged micrographs (Figure 1F). The line drawn through Figures 1D, E, F, clearly demarcates the highest accumulation of SMAA expressing cells in the stratum granulosum and its absence in stratum corneum of young human foreskin (Figure 1E) which strongly stained for GS (Figure 1D). GS and SMAA were both present in stratum granulosum and inner parts of epidermis (Figure 1F). In foreskin dermis, on the other hand, SMAA (red, Figure 1E) could barely be detected in fibroblasts moderately and evenly expressing GS (green, Figures 1A, C, D, F). Instead, it was strongly expressed in myofibroblasts surrounding the middle-sized vessels (yellow arrows in Figure 1E, F) and in the papillary zone of the dermis in which GS was poorly presented (orange staining in merged Figure 1F). GS and SMAA were also co-localized in association to large vessels situated in the reticular part of the dermis (not shown).
Co-localization of GS and β-catenin in aged human temple skin.
Since the Wnt/ß-catenin signalling pathway was recently found to play an important role in the regulation and zonal expression of GS in liver [31], [32] we wondered whether ß-catenin might be co-localized with GS in skin as well. Figure 2A shows conventional eosin staining of temple skin of aged (70-year-old) male patient. Immunohistological staining of this region of aged skin with a monoclonal anti-GS-antibody and peroxidase (POD)-coupled secondary antibodies revealed the presence of GS in epidermis (Figure 2B). In aged human temple skin, the staining for GS was especially strong in stratum granulosum, while it was almost absent from the utmost layer of stratum corneum. β-catenin, was relatively strongly expressed in cells of stratum basale and stratum spinosum (Figure 2C). In stratum granulosum the intensity of β-catenin staining abruptly decreased. Some keratinocytes expressed β-catenin preferentially in the membranes and slightly in the cytoplasm but not in the nucleus, whereas in other keratinocytes a faint staining of the nuclei could be observed. The heterogeneity in staining for β-catenin and its intercellular localization may be explained by differences in the individual rates of differentiation of keratinocytes, as well as by region-specific requirements. Remarkably, GS (at a moderate level) and β-catenin were both present in stratum basale, the actual proliferative compartment, and in stratum spinosum.
(A) hematoxiline staining of a skin sample. Stratum basale can be identified by cells with prominent nuclei. (B) GS is localized throughout the viable part of the epidermis. The highest staining intensity can be detected at the interface of stratum granulosum and stratum corneum. (C) Localization of β-catenin in lower parts of the epidermis. β-catenin shows a strong membraneous and cytoplasmic staining in stratum basale and in stratum spinosum. Arrows in (C) point to the presence of catenin in the nucleus of keratinocytes. Scale bar 25 μm.
Age-specific and regional distribution of GS and GFAP in rat skin.
When skin samples of newborn and adult rats were compared, it became obvious that immediately after birth GS is strongly expressed in stratum basale of rat scalp and much less intense in dermal fibroblasts as shown by confocal laser scanning (CLS) micrographs of newborn rat scalp sections (white arrows Figure 3A, B). In hair follicles of newborn rat scalp, GS was prominent in the outer sheet and in the medulla (red arrows in Figures 3E–G). CLS microscopy of culture-activated fibroblasts isolated from young human skin showed strong reaction of GS in cytoplasm and especially nuclei of the cells (yellow arrows in Figures 3D, H).
(A) Representative of serial optical sections obtained by CLS microscopy of newborn rat skin stained for GS (green). (B) Phase contrast micrograph of the field shown in (A). (C) Wide-field fluorescence microscopy of fibroblasts in human skin. (D, H) Representative of serial optical sections obtained by CLS microscopy of cultured human fibroblasts stained for GS. GS was detected using rabbit antiserum and FITC-conjugated goat anti-rabbit IgG. (E, F) Representatives of serial optical sections obtained by CLS microscopy of hair follicle in newborn rat skin section stained for GS. (G) Phase contrast micrograph of the field shown in E and F. Blue arrows point to epidermis, magenta arrows to the keratinocytes forming the stratum basale of the epidermis, white arrows to fibroblasts, green arrows to the outer sheet of the hair follicle, red arrows to the hair channel. Scale bar in (A, B, D, H) 20 μm; in (C) 100 μm; in (E, F, G) 40 μm.
After few days, i.e., in 2–3-day-old rat scalp sections GS was found in all layers of epidermis. GS expression (green) was significantly increased in stratum granulosum (magenta arrows in Figure 4A–C) and was present in corneocytes in some regions of stratum corneum (yellow arrows Fig 4A–C) which at that time still contained many nuclei or nuclear remnants revealed by 4′,6 diamidino-2-phenylindole (DAPI) staining. At this age, co-localization of GS (green) with GFAP (red) in stratum corneum was less prominent than in stratum granulosum (cf. magenta and yellow arrows in Figure 4C). By contrast, in adult rat scalp staining intensity of GS at the interface of stratum granulosum and stratum corneum decreased (Figure 4D), whereas in the same region GFAP dominated (white arrows in merged Figure 4F). In adult rat scalp sections, the number of nuclear remnants in stratum corneum was strongly decreased compared to aged skin in humans. Though this type of co-localization of GS and GFAP was preserved in other skin samples of adult rats, for instance in leg skin (Figure 4G–L), the ratio between GS (green) and GFAP (red) seemed to vary slightly depending on whether samples from lateral (Figure 4G–I) or medial (Figure 4J–L) leg skin were stained. Thus, in the lateral surface of the leg skin many regions lacking GS (white arrows in Figure 4G–I) could be found, whereas in medial surface of the leg skin the GS/GFAP ratio was significantly increased (red arrows in Figure 4G–L).
(A–C) Double labelling of newborn (2–3-day-old) rat scalp. (A) staining for GS (green, pAb), (B) staining for GFAP (red, mAb), (C) merge. (D–F) Double staining of adult rat scalp sections. (D) staining for GS, (E) staining for GFAP, (F) merge. The insert in (C) shows single keratinocytes strongly stained for GS. White arrowheads in the insert point to GS-positive cells migrating towards the outer layer of the skin. The insert in (F) shows the prominent differences in the ratio of GS and GFAP in neighboring regions of the epidermis of adult rat skin evidenced by green, yellow or orange staining. Red arrows in (A–F) point to stratum basale, white arrows to stratum spinosum, magenta arrows to stratum granulosum, yellow arrows to stratum corneum. (G–L) Co-expression of GS and GFAP in adult rat leg skin. (G–I) Double labelling of skin section from the lateral surface of adult rat leg skin. (G) staining for GS (green, pAb), (H) staining for GFAP (red, mAb), (I) merge. (J–L) Double staining of skin section from the medial surface of adult rat leg skin. (J) staining for GS, (K) staining for GFAP, (L) merge. White arrows in (G–L) point to the portion of the skin in which GS can be barely detected, whereas red arrows point to the portion of the skin in which GS is strongly expressed. Binding of specific antibodies was visualized with FITC-conjugated goat anti-rabbit IgG (A, D, G, J) and Cy3-conjugated goat anti-mouse IgG (B, E, H, K). Scale bar: (A–C) 10 μm; (D–F) 20 μm.
Co-localization of GS and metallothionein in skin slices and cultured cells.
The pattern of staining for metallothionein (MT) in newborn rat scalp (Figure 5A, B) was different from that of in human skin described previously [21]. In human skin, keratinocytes strongly expressing MT in all layers of epidermis exhibited widespread co-localization with GS. By contrast, in newborn rats, the only region of the epidermis reacting with mAb MT (red) was the stratum basale (magenta arrows in Figure 5A). Only in this layer of epidermis, GS (green) showed some co-localization with MT. In rat scalp skin dermis, GS and MT were localized in functionally different dermal cells. MT (red) was evenly distributed in GS-negative fibroblasts throughout the dermis (white arrows in Figures 5A, B), whereas GS was prominent in the outer sheet (green arrows in Figure 5A, B) and medulla of hair follicles (red arrows in Figure 5A, B). Though weakly, GS was also expressed in the sweat glands (yellow arrowheads in Figure 5B). MT and GS were also present in germinative epidermal cells located in the lower end bulb region of rat hair follicles (yellow arrows in Figure 5B).
(A, B) Double-staining for GS (green) and MT (red) in newborn ratscalp sections. (B) Expression of GS (green) and MT (red) in rat scalp hair follicle. Cell nuclei in A–L are stained with DAPI (blue). (C) Co-expression of GS (green) and MT (red) by cultured newborn rat astroglial cells. (D–F) Expression of GS (D) and MT (E) and their co-localization (F, merge) in cultured human skin keratinocytes. GS was detected using rabbit antiserum and FITC-conjugated goat anti-rabbit IgG, whereas MT was detected using mAb MT and Cy3-conjugated goat anti-mouse IgG. Blue arrows point to stratum corneum, yellow arrows in (A) to stratum basale, magenta arrows to the keratinocytes forming the stratum granulosum, red arrows in A and B to the hair channel, green arrows to the outer sheet of the hair follicle, white arrows to fibroblasts; yellow arrowheads in (B) to sweet glands. Red arrows in (D–F) point to cells which predominantly express MT, green arrows in (D–F) point to cells which predominantly express GS. Scale bar: in (A, D, E, F) 10 μm; in (B, C) 20 μm.
When human keratinocytes were brought to culture, they maintained a strong staining for GS for 6 days (Figure 5D). Simultaneously, they expressed MT (Figure 5E) evidenced by overlapping yellow stain in merged micrograph (Figure 5F). However, different cells could be observed which expressed GS stronger than MT (green arrows in Figures 5D–F) and vice versa (red arrows in Figures 5D–F). The heterogeneity in the intensity of staining of GS and MT in neighbouring keratinocytes was comparable with that of rat astroglial cells (cf. Figures 5F and 5C). This fact further evidenced the specificity of antigen recognition by the anti-GS antisera and mAb against MT.
Factors influencing GS expression and activity in skin
HaCaT cells.
Regulatory features of GS were investigated in primary human keratinocytes and particularly in HaCaT cells, a spontaneously immortalized human keratinocyte cell line [33] in which the GS activity was only slightly higher compared to primary human keratinocytes. Thus, the specific activity of GS in primary human keratinocytes cultured for 24 h amounted to 4.3±1.8 mU/mg protein (Table 1), whereas the average GS activity in HaCaT cells amounted to 6.8±4.8 mU/mg protein (Table 1). difference between the primary cells and the HaCaT cells was statistically insignificant due to the high variation of the activity in this cell line.
Cell density/glutamine.
Careful investigation of this variability revealed that GS activity in the growing HaCaT cell line was considerably influenced by the cell density as well as by the glutamine content of the culture medium. Other differences between the culture media seemed of less importance. When HaCaT cells were cultivated for 24 h in the absence of Gln, GS activity was approximately 2-fold higher than in the presence of 5 mM Gln (Figure 6A). While the higher activity in the absence of Gln remained nearly constant for 96h, the initially low activity in the presence of Gln slightly increased with time in parallel to the sustained cell growth under these conditions. Accordingly, when HaCaT cells were plated at low cell density, GS activity was very low (Figure 6B). During prolonged cultivation (>96 h), again, there was a steady increase in specific activity of GS as cell density increased. After 168 h, when cell layers had reached confluence and were highly packed, GS activity increased dramatically (Figure 6B) indicating that intensive cell-to-cell interactions are an important factor for high GS expression in this cell line.
(A) Effect of Gln on the specific activity of GS. Cells were cultivated over 96 h with (squares) and w/o (circles) 5 mM Gln. Medium was renewed every day. Each point represents the mean±SD of 3 determinations for a representative culture. (B) Effect of cultivation time on the specific activity of GS. Cells were cultivated for the times indicated and then harvested. Culture medium was exchanged 3 times a week. Each point represents the mean±SD of 3 determinations for a representative culture. (C) Effect of dexamethasone on the specific activity of GS. Cells were incubated with the indicated concentrations of dexamethasone for 24 h. Each point represents the mean±SD of 3 determinations. (D) Effect of ammonium chloride on the specific activity of GS. Cells were incubated for 24 h in the presence of the indicated concentrations of NH4Cl. Each point represents the mean±SD of 3 determinations for a representative culture. Statistically significant from controls: *, p<0.05; **, p<0.01; ***, p<0.001.
Dexamethasone.
As found with many cell lines [31], [34], [35], the synthetic glucocorticoid dexamethasone strongly (8-fold) induced the activity GS in HaCaT cells (Table 1). Examining of the concentration-dependency of this effect revealed that maximal induction in the HaCaT cells was reached above 0.1 μM dexamethasone (Figure 6C). Partially, this induction occurred at the transcriptional level, because GS mRNA determined by quantitative reverse transcriptase polymerase chain reaction (RT-PCR) increased 2.38-fold±0.38 (N = 3; p<0.05) after induction by 1 μM dexamethasone within 24 h (Table 1). Surprisingly, primary keratinocyte culture did not respond. Whether this may be due to the fact that keratinocyte growth medium contains hydrocortisone and, thus, primary cells might already reflect a somewhat induced state remains to be determined. Since hydrocortisone is vital for maintaining primary keratinocytes in culture, this hypothesis cannot directly be tested experimentally.
Ammonium ions.
A rather unexpected finding obtained using HaCaT cells was that GS activity strongly increased in response to exposure to NH4+ ions. Depending on the specific activity of controls an increase in GS activity, up to approx. 9-fold, could be observed after the addition of 30 mM NH4Cl (Table 1). Figure 6D shows the concentration-dependence of this effect. Even in dense cultures showing a high control activity such as depicted in concentrations as low as 5 mM NH4Cl (Figure 6D) caused a significant increase in specific GS activity within 24 h. Generally, exposure to high concentrations of NH4Cl led to the highest GS activites around 80 mU/mg protein measured in HaCaT cell cultures. Even at concentrations as high as 30 mM NH4Cl no changes in cells size or shape were visible in bright field microscopy. In contrast to enzyme activity, the increase in GS mRNA over controls determined by quantitative RT-PCR under all conditions was insignificant. For instance, in the presence of 30 mM NH4Cl the fold increase of GS mRNA amounted only to 1.45±0.28 (N = 4). GS activity in primary human keratinocytes similarly responded to ammonium ions (Table 1), although the increase was less prominent compared to the cell line. Absence of alteration in molecular activity of the enzyme under these conditions (not shown) excluded posttranslational modification. These findings suggest a marked posttranscriptional influence of NH4Cl on GS, similar to that described in skeletal muscles [36].
Lithium chloride.
In order to learn more about the possible involvement of β-catenin signalling in the regulation of GS in skin, we exposed cultured human keratinocytes and HaCaT cells to LiCl, a commonly used glycogen synthase kinase 3ß (GSK3β) inhibitor [37] that is able to activate β-catenin and to induce GS in hepatocellular populations [38], [31]. As shown in Table 1, LiCl failed to significantly induce GS in both types of cells, although activity values tended to be slightly increased. Thus, β-catenin signalling may be necessary, but not sufficient for reaching high levels of GS protein in keratinocytes.
Discussion
Cellular localization of GS in skin and its correlation with neural marker proteins
The present study demonstrates the previously unknown distribution of GS in human and rat skin. It shows unexpectedly large stores of GS in epidermal keratinocytes in human and rat skin sections. This study contradict to low activity of this enzyme in rat and murine skin homogenates demonstrated in very few reports elucidating the presence of GS in normal skin [14], [16]. The accumulation of GS in all epidermal cell layers was detected using mAB and pAb against GS. The authenticity of antigens recognized by pAb GS is confirmed also by heterogeneity in the intensity and pattern of GS staining between neighboring cells and regions of epidermis and dermis, as well as between cultured human keratinocytes, that might be due to differences in the individual rates of differentiation of these cells. The expression of GS throughout all layers of the epidermis suggests its importance for several skin-specific functions (see Table 2). Thus, the presence of GS in stratum basale suggests its involvement in sustained rejuvenation of keratinocyte population, its accumulation in stratum granulosum may indicate its involvement in the establishment of the epidermal permeability barrier, whereas its prominent expression in the outermost layer of the epidermis, the stratum corneum may hint at its necessity for the physical and chemical defense [39]. The loss of these functions as observed in inherited GS deficiency [17] could explain the severe skin pathology associated with this disease.
GS and epidermal permeability barrier
GS is related to proteins involved in establishment of protective barriers against external signals at the blood-tissue interfaces in brain and liver. The present study shows that GS is essential also for establishment of epidermal permeability barrier. The large amount of GS throughout the epidermis and also in dermis is in agreement with the main function of skin to control the homeostasis of the organism. The intimate connection of Gln-enriched proteins to an epidermal barrier function has been proven in human skin diseases [40] and in transgenic mice overexpressing claudin-6, i.e., tight junction protein in the epidermis [41]. Therefore, keratinocytes of stratum granulosum carry a particular burden, because in this layer cells synthesize lots of proteins and other material important for terminal differentiation of keratinocytes into corneocytes and generation of the stratum corneum. Many of structural proteins involved in establishment of epidermal barrier for example involucrin, loricrin, and filaggrin, contain a disproportionally high percentage of Gln [41]–[44] and are increased during development of epidermal barrier [41], [45]. Thus, synthesis of skin proteins creates a strong demand for enhanced intracellular pool of Gln that most likely cannot be satisfied by diffusion of Gln from the blood through stratum basale and stratum spinosum. Consequently, high local production based on the predominant expression of GS in stratum granulosum and the adjacent part of stratum corneum may be of utmost importance to guarantee an optimal supply of Gln.
An epidermal barrier is in part formed by tight junction components which in adults are localized to a narrow zone of the granular cells [46]. Strong expression of GS in stratum granulosum and stratum corneum of young human skin and its redistribution into the stratum granulosum and inner layers of the epidermis in senile human skin shown in the present study might reflect its active involvement in protection provided by tight junctions. Indeed, GS has been shown to prevent disruption of the tight junctions by acetaldehyde, to maintain the transepithelial resistance and to decrease the paracellular permeability [28]. Furthermore, exposure of intestinal cell cultures to Gln influenced the expression of functional components of tight junctions, i.e., claudin-1, occludin, and ZO-1 protein [29].
The timing of GS expression in keratinocytes coincides with production of MT, another proliferation-inducing and barrier supporting factor [47]. Presence of MT in different cell types evidence their capacity to reflect the attack of immunologic stressors, oxidative stress and intoxication caused by heavy metals [48]. The co-localization of GS and MT has been shown also in functionally active astrocytes and activated HSC [7], [9], [21], [22]. In the light of elevated occurrence of cadmium in the environment and increased human use of this toxic heavy metal [49], a further role for MT in skin specific functions may be related to protection against cadmium-induced damage of tight junctions [50], [51]. After being trapped by metallothionein, ionic cadmium [Cd2+] lost its capacity to damage the tight junctions between LLC-PK1 cells [50]. Co-production of GS and MT by young human foreskin epidermal cells and especially by keratinocytes situated in the stratum basale of newborn rat skin is in accordance with literature data showing direct correlation between neural and non-neural cell proliferation rates and concentrations of MT [23] and GS [12], [22], [52].
Actin cytoskeleton plays an essential role nearly in all functions performed by skin, i.e., cell division [53], contraction [54], migration [55], [56] and stratification of epidermis [57]. SMAA, the marker protein of myofibroblasts, is also related to junction-associated proteins [58], [59]. In active states of the GFAP-positive HSC, mesangial cells, astrocytes characterized by increased capacity for proliferation and resistance to environmental insults SMAA is contracted to the perinuclear area [23], [24] similar to that of observed in keratinocytes. Simultaneous appearance of SMAA, GS and MT at functionally active states of astrocytes, HSC, mesangial cells and keratinocytes [21], [23], [24]. further emphasizes our hypothesis of the commonness of mechanisms operating at the border of different environments and tissues, in particular at the integumentum. Functional association between actin, tight junction, adherens junction proteins and GS were evidenced by reduced acetaldehyde-induced dissociation of occludin, zonula occludens-1, E-cadherin, and beta-catenin from the actin cytoskeleton when Caco-2 cells were exposed to Gln [28]. In this study, an indirect evidence of functional association of actin with mechanical barrier provided by tight junction [58]–[60] is presented by dense lining of actin-positive cells in stratum granulosum of young human foreskin. A week SMAA immunoreaction and moderate mRNA have been shown in a small number of keratinocytes in the interscapular region of intact newborn rat skin [61]. Furthermore, in a current study on adult murine skin we found that the number of SMAA-synthesizing keratinocytes was strongly dependent on the strain of mice and was sometimes lower than in human skin (unpublished results).
Epidermal keratinocytes are faced with the complex task of providing anti-cytotoxic and mechanical defense supported by SMAA cytoskeleton, as well as facilitated exchange with external environment and immune barriers supported by GFAP cytoskeleton. High levels of filamentous GFAP expression in differentiated astrocytes and non-differentiated HSC and mesangial cells were associated with cellular functions associated with facilitated transport and down-regulation or absence of GS, MT and SMAA [23], [24], [62]. Therefore, co-expression of GFAP and major histocompatibility complex II by keratinocytes [21] on the one hand, and of MT, SMAA and GS on the other hand, is a further evidence of complex tasks of keratinocytes to distinguish between external signals to be utilized from those to be blocked. Further studies are necessary to understand the enigma of appearance of SMAA, the marker protein of myofibroblasts and mesenchyma cells, in epidermal keratinocytes.
Age associated changes of GS
The balance between growth and apoptosis of keratinocyte providing continuous renewal and resistance of stratum corneum to external signals is disturbed with age. The mechanisms involved in this process are not well understood. Our study shows that production of GS by skin is developmentally regulated and that the dynamics of postnatal differentiation of GS in human and rat skin is comparable with age-dependent changes in GS expression in human and rat skin (Table 2). Both in humans and rats aging of the skin led to accumulation of GS in stratum granulosum and downregulation of the enzyme in stratum basale. Presence of GS in newly formed corneocytes which at that time still contained many nuclei evidenced the importance of GS for functions performed by living cells. Likewise, in young foreskin which showed the smallest number of stratum corneum cell layers GS was found in all layers. By contrast, the stratum corneum of aged human temple skin which demonstrated multiple layers of cells in stratum corneum was devoid of GS. The data presented further suggest that GS is always associated with developing keratinocytes up to the stage of terminal differentiation of the corneocytes that results in programmed cell death partially resembling apoptosis [63], [64]. The differences observed in stratum corneum cell layers depending on location, age and among different individuals corroborate previous findings [26] demonstrating the smallest number of stratum corneum cell layers in genital skin compared to that of face and scalp.
In accordance with studies demonstrating age-dependent decrease in the permeability barrier of the skin and seized capacity of skin stem cells for repair with age [25], [65], [66], strong expression of GS in newborn rat skin stratum basale, consisting mainly of stem cells, slightly decreased in adult animals. Also the intense staining for GS throughout the epidermis of young human foreskin implies high potency of this skin region for proliferation and regeneration. The presence of β-catenin in inner layers (spinous and granular layers) of aged skin epidermis shown herein demonstrates the upkeeping of the stem cell pool in elderly [67]. Changes in the architecture of senile human skin were illustrated not only by absence of GS and thickening of stratum corneum but also by dense laying of keratinocytes intensely stained for GS in stratum granulosum. Whether the redistribution of GS from stratum corneum to stratum granulosum, a region enriched by tight junction-associated proteins [58], [46], reflects an age-associated dehydration leading to laxity and changes in the architecture of the skin [68] is a matter of future investigations.
Simultaneous presence of GS and β-catenin in keratinocytes of stratum basale and stratum spinosum and the presence of activated cytoplasmic and nuclear β-catenin in these cells shows similarities to the regulation of GS expression in hepatocytes. There, active Wnt/β-catenin signalling is required for initiating GS expression [31], [32], [38]. Our findings concerning co-localization of β-catenin and GS suggests that the mechanism of post differentiation patterning recently hypothesized for liver tissue [31] may likewise be relevant for skin. Briefly, post differentiation patterning suggests that β-catenin signalling acts on proliferating or differentiating cells imprinting them to express GS and rendering this expression to be regulated by various other signals. These features are then maintained in quiescent, post-mitotic cells even in the absence of continuous β-catenin signalling and allow extremely high expression levels of this enzyme [31]. Exactly this situation seems to occur when keratinocytes terminally differentiate in stratum granulosum where no activated β-catenin was found, but the highest concentration of GS is reached.
Ammonium ions as regulators of GS activity
The regulatory mechanisms controlling the GS activity in skin present a mixture of mechanisms controlling this enzyme in inner organs with an unusual mode of regulation by ammonium ions, pointing to hidden mission of this enzyme in the integumentum. Liver and brain are the major ammonia consuming systems metabolizing it to Gln [69]. Among mechanisms triggering blood-brain barrier alterations in hepatic encephalopathy and its reestablishment after reversal of fibrosis, the central place is given to hemodynamic changes and circulating ammonia [70], [71]. GS prevents the entry of high amounts of ammonia from circulation to brain and thus, attenuates neurotoxicity. The changes in the distribution of this critical enzyme suggest that the glutamate-glutamine cycle may be differentially impaired in hyperammonemic states [72]. Both brain and liver reacted to hyperammonemia by down-regulation of GS [68], a response that was also found in cultured hepatocytes [3]. In contrast, skeletal muscles react to increase in blood ammonia level by up-regulation of GS [73]. In skeletal muscle, enzymatic activity (but not gene) was significantly up-regulated [36], [68], [73], [74]. In the hyperammonemic rat muscle ammonia levels were always increased and muscle Gln decreased, probably indicating glutamate consumption by enhanced Gln synthesis [75].
Recent studies showed that ammonia was present in gas emanated from the skin surface of healthy persons and patients with hepatic disease. The average level of ammonium ions removed via skin correlated with that of in blood and it reached the highest amounts in so-called skin gas collected from patients with hepatic disease [76]. This mode of elimination of circulating ammonia may contribute to and partially explain the large amounts of GS in the skin. Judging from the fact that erythema could be induced when highly ammoniacal urine was applied exclusively to scarified skin [77], the roots of the severe skin pathology in GS-deficiency [17] primary lay in deficit of Gln leading to reduced production of structural proteins. In the light of our results demonstrating the GS-activating effect of ammonia, the removal of circulating ammonia via skin presents a natural continuously acting mechanism of regulation of GS activity favoring the local skin requirements for Gln in normal physiological conditions as well as in pathologic situation. Large amounts of GS in keratinocytes in situ and in culture and over-activation of GS (but not mRNA) in cultured keratinocytes exposed to ammonium ions, allows to consider the skin as powerful ammonium detoxification pool which comes to action during hyperammonemia. On the other hand, it is well established that hyperammonemia may disrupt blood-brain barrier integrity [78]. Also Madin-Darby canine kidney cells responded to elevated extracellular NH4Cl concentrations by distinct alterations in the architecture and transepithelial transport properties, redistribution of occludin, a tight junction protein, and reorganization of the actin cytoskeleton [79]. Therefore, the continuous irrigation of normal epidermis with small amounts of circulating ammonia may play a positive role not only in the sense of activation of GS, but also in preservation of exchange between the skin and external world.
Other factors regulating the GS activity
The presence of ornithine aminotransferase in skin [80] renders it possible that a similarly efficient production chain for Gln exists in epidermal keratinocytes as it is found in pericentral hepatocytes, the predominant site of Gln formation in the liver [31]. Nonetheless, further mechanisms seem to exist which can enhance GS activity, in order to match the need for an extraordinary high Gln synthetic capacity in certain skin layers. Regulation of keratinocytic GS by glucocorticoids and Gln shows many features known for other cells, e.g. astrocytes [81]–[84]. The same is true for regulation of GS by the density of keratinocytes. Naturally, high density of cultured keratinocytes provides higher level of GS, therefore of Gln, an amino acid known to induce the proliferation of different cell types. Also GS activity of liver-derived epitheloid cell lines and astrocytes is upregulated with increasing cell density and peaks in confluent cultures [34], [85].
Extrapolating the results obtained on cultured skin cells into in vivo conditions allows to propose that epidermal permeability barrier depends on Gln-induced expansion of keratinocytes that in turn increases the density of cell sealing and logically limits the paracellular permeability. The findings reported herein for keratinocytes contrast with those reported for dermal fibroblasts [86]. Thus, despite the presence of GS in many cell types of the skin, this organ does not seem to act uniformly with respect to GS expression and Gln synthesis, but rather shows considerable heterogeneity tailored to serve complex skin-specific functions.
Concluding remarks
The present study comprises several experiments opening a new view on the physiological importance and multiple roles of GS in a complex series of events foreseen by an epidermal program aiming at the establishment of epidermal permeability barrier supported by sustained rejuvenation, differentiation, transepithelial resistance, detoxification, immune protection and cell-to-cell interactions. Since GS expression in skin is developmentally regulated, it may, thus, additionally be involved in mechanisms regulating the balance between cellular growth and programmed cell death.
Our study suggests that the apparently low activity of this enzyme in skin was previously underestimated resulting from measurements of average enzymatic activity in whole skin homogenates containing both enzymatically active and silent GS. These studies neglect the local skin-specific cellular functions and undervalued the capacity of keratinocytic GS for being modulated in health and disease. The results reported here in conjunction with literature data open new perspectives in the investigation of skin cell functions in healthy and pathological states. They call for further elucidation of the functional predestination of large stores of immunoreactive but enzymatically silent GS in epidermis particularly in stratum corneum as well as of regulatory mechanisms controlling its enzymatic activity, and especially of the role of circulating ammonia in establishment of the epidermal permeability barrier. Thus our results favor not only local specific functions of GS comprising the production of excess Gln for regional biosynthetic purposes, they also suggest a life-essential role of keratinocytic GS for whole organism in health and disease.
Materials and Methods
Reagents.
Dexamethasone, Gln, penicillin, streptomycin, POD-extravidin, diaminobenzidine, aminotriazole, goat serum and Triton X-100 were products of Sigma (Taufkirchen, Germany). NH4Cl, ethylenediaminetetraacetic acid (EDTA), H2O2, Roti-Histokit, Tween 20 were purchased from Roth (Karlsruhe, Germany). Oligo(dT) primer, primer for GS and β-actin, Superscript II Reverse Transcriptase, SeeBlue® Pre-Stained protein standards were products of Invitrogen GmbH (Karlsruhe, Germany). The culture medium Dulbecco's modified Eagles medium (DMEM) and fetal calf serum (FCS) were purchased from GIBCO (Eggenstein, Germany). Keratinocyte growth medium and human epidermal growth factor (Clonetics, USA), trypsin and the Light Cycler FastStart DNA Master+SYBR Green I Kit were products of Roche Diagnostics GmbH (Mannheim, Germany). Vectashield mounting medium was purchased from Vector Laboratories (Burlingame, CA, USA). RNA isolation was performed using the Nucleo Spin RNA II Kit from Macherey-Nagel (Düren, Germany). Cell culture material was obtained from Techno Plastic Products AG (Trasadingen, Switzerland) as well as from Greiner Bio-One GmbH (Frickenhausen, Germany).
Antibodies.
Monoclonal mouse anti-GS and monoclonal mouse anti-β-catenin antibodies were products of Becton, Dickinson and Company Transduction Laboratories (Heidelberg, Germany). Goat anti-mouse IgG Fab–POD fragment was purchased from Sigma (Taufkirchen, Germany). Biotinylated goat anti-mouse IgG-Fc antibody and sheep anti-mouse IgG Fab-AP were products of Chemicon International Ltd. (Hampshire, United Kingdom). Monoclonal anti-GFAP (clone GF 12.24) and monoclonal antibody against SMAA (anti-SMAA, clone ASM-1) were products of Progen Biotechnik GmbH (Heidelberg, Germany). The monoclonal antibody against Cd/Zn-inducible MT-1 was a generous gift of Prof. U. Weser (University of Tübingen, Germany). Polyclonal anti-GS antibody against pig brain GS was raised in the laboratory of Dr. Jaenicke [87]. Fluorescein isothiocyanate (FITC)-conjugated goat anti-rabbit IgG and Cy3-conjugated goat anti-mouse IgG were from Dianova Jackson Immuno-research (West Grove, USA).
Animals.
New-born and adult Sprague-Dawley rats (250 to 300g) were obtained from Charles River (Sulzfeld, Germany) and maintained at the central animal facility according to institutional guidelines for ethical care of animals. Samples of rat skin were prepared from the scalp of newborn rats after extirpation of the brain which was used for the preparation of astroglial primary cultures.
Human skin.
Samples of human foreskin were obtained from the Childrens Hospital of the University of Leipzig with consent from patients who underwent circumscission (phimosis) and samples of temple skin of 70-year-old male (healthy border of a basal cell carcinoma) from the Dermatology department of the University of Leipzig. All human skin samples were taken after written consent of the patients and in accordance with the principles and under the license of the Ethic Commission of the University of Leipzig.
Cell culture
Primary keratinocyte culture.
Primary normal human epidermal keratinocytes were isolated from the foreskins of 2–8 year old children according to the methods described by Zellmer and Reissig [88]. Briefly, the cells were seeded in Petri dishes and were grown in serum-free keratinocyte growth medium supplemented with 0.15 mM CaCl2, 0.1 μg/ml human epidermal growth factor, 0.5 μg/ml hydrocortisone, 5 μg/ml insulin, 30 μg/ml bovine pituitary extract, 50 μg/ml gentamycin, and 50 μg/ml amphotericin. Cultures were terminated at day 7 as described previously [21].
Keratinocyte cell line.
HaCaT cells [33] were cultivated using DMEM medium supplemented with 2 mM glutamine, 10% FCS, 50 U/ml penicillin and 37.5 U/ml streptomycin in 75 cm2 cell culture flasks. For sub-cultivation the cells were incubated with Hanks balanced solution without calcium, supplemented with 0.05% EDTA for 20 minutes. Then, cells were harvested using a Hanks solution composed of 0.05% trypsin and 0.025% EDTA and suspended in supplemented DMEM.
Fibroblasts.
Monolayers of normal human dermal fibroblasts from the foreskins of 2–8 year old children were obtained from explant cultures of de-epidermized skin and cultured in DMEM containing 10% heat-inactivated FCS (Gibco, Karlsruhe, Germany), 50 μg/ml L-ascorbic acid, 100 U/ml penicillin, and 100 μg/ml streptomycin sulphate, as previously described [89]. The fibroblast cultures were kept in an incubator with 5% CO2 in air (95% humidity) at 37 °C. Cultures were terminated at day 1 and 3 in culture as described previously [21].
Astroglial cells.
Rat astroglia-rich primary cultures were prepared from brains of newborn animals as described elsewhere [90].
Immunohistochemistry and Immunocytochemistry
Indirect double- and mono immunofluorescence studies.
Unfixed 7 μm cryostat human and rat skin sections, cultured human keratinocytes and fibroblasts, as well as cultured rat astroglial cells were prepared as described previously [91]. After fixation in methanol (−20°C), the cells and tissue slices were washed with phosphate buffered saline (PBS) at room temperature (RT). In monolabelling studies, the sections and cells were exposed to pAb anti-GS (dilution 1∶100) only. In double-immunolabelling studies, mixtures of pAb anti-GS with mAb against GFAP (dilution 1∶100) or mAb against Cd/Zn-inducible MT-1 (1.7 μg/μl, dilution 1∶100) [7], [23], [92], or mAb against SMAA (dilution 1∶100) were applied. After 2 h incubation at RT, specimens were washed and exposed for 1 h at RT to a mixture of the secondary antibodies: FITC-conjugated anti-rabbit IgG (dilution 1∶100) and Cy-3 conjugated anti-mouse IgG (dilution 1∶800). All antibodies were diluted with PBS. Subsequently, the cells and tissues were washed with PBS containing Triton X-100 and mounted in Vectashield mounting medium with or w/o DAPI.
Immunochemical detection of GS and β-catenin.
Human skin samples were stored at −80 °C. Slices were cut and fixed in 3.5% paraformaldehyde immediately before staining. For the detection of β-catenin the tissue slices were permeabilized with 0.1 M Tris-borate buffer (pH 7.4) containing 0.2% Tween20 and the endogenous peroxidase activity was destroyed by incubation with 0.3% H2O2. The slices were incubated with monoclonal mouse anti-β-catenin antibody over night. After washing the secondary biotinylated goat anti-mouse IgG-Fc antibody was added for 1 h at RT followed by addition of the POD-Extravidin complex for 30 min. Staining was performed in 0.1 M Tris-HCl buffer (pH 7.6), composed of 0.05% diaminobenzidine, 2% aminotriazole and 0.033% H2O2. Finally the slices were dehydrated and embedded using Roti-Histokit. For the detection of GS the tissue slices were fixed and permeabilized as described for β-catenin staining. Non-specific binding sites were blocked with 10% goat serum and the slices were incubated with monoclonal mouse anti-GS antibody at 4°C over night. Subsequently the slices were washed and incubated with a goat anti-mouse IgG Fab–POD fragment. Staining and embedding was performed using Roti-Histokit. Nuclei were stained by immersion in Haemalaun solution for 2 min followed by washing for 10 min with tap water.
Microscopy
Bright field microscopy.
POD-labelled sections were visualized using a Leica DM5000 B microscope (Leica, Bensheim, Germany) equipped with a HCX PlanApo 40×/0.75 objective and a Leica FX 350 camera using the LAS software of Leica.
Fluorescence microscopy.
FITC-conjugated anti-rabbit IgG-labelled and Cy-3 conjugated anti-mouse IgG-labelled sections and cells were examined using:
- Wide-field fluorescence microscope BX 51 (Olympus Optical Co. Europe, Hamburg, Germany) with UplanFI 20×/0.5 Ph1, UPlanFI 10×/0.30 Ph1, and UPlanFI 40×/0.75 Ph2 objectives. Images were taken with the digital camera F-View II (Soft Imaging System, Leinfelden-Echterdingen, Germany) and data were processed with AnalySIS DOKU® (Soft Imaging System).
- Confocal laser scanning microscope Leica SL equipped with an argon/krypton laser (Leica Lasertechnik, Heidelberg, Germany). To improve the signal-to-noise ratio, 8 scans of one focal plane were averaged. The confocal image data were obtained using a PLANAPO 63×, 1.32 NA oil immersion objective and confocal laser scanning microscope software (Leica Lasertechnik), and processed with Adobe Photoshop 7.0 software (Adobe Systems Inc., Mountain View, CA, USA).
Determination of glutamine synthetase activity
Specific GS activity was determined by the method of Levintow [93] with minor modifications described by Gebhardt and Williams [94]. Briefly, 7.5×106 cells were seeded into 6 well plates and cultivated in 1 ml medium at 37°C and 5% CO2. After washing with Hanks balanced solution the cells were harvested using a rubber police man, disrupted by sonication (Sonoplus, Bandelin, Germany) and the protein concentration was determined according to Bradford [95] in order to calculate the specific GS activity.
Quantitative PCR
Cells were washed twice with Hanks balanced salt solution. Total RNA was isolated using the Nucleo Spin RNA II Kit according to the manufacturer description which included DNase I digestion. One μg of total RNA was reverse transcribed using oligo(dT) primer and Superscript II Reverse Transcriptase. The cDNA was diluted 1/10 and 3 μl were used for amplification of GS and β-actin as internal control using the Light Cycler FastStart DNA MasterPLUS SYBR Green I Kit. The following primers were used for GS: 5′-CACTACCGGGCCTGCTTGTAT-3′ (forward primer) and 5′-GCATGGCCTTGGTGCTAAAGTTG-3′ (reverse primer), for β-actin: 5′-AGAAAATCTGGCACCACACC-3′ (forward primer) and 5′-CTCCTTAATGTCACGCAC-GA-3′ (reverse primer). The PCR reactions were performed in duplicate in 20 μl volume containing 3 μl cDNA, 0.5 μM of each primer, and 4.0 μl 5×Master Mix. PCR products were quantified using a Light Cycler 2.0 (Roche Diagnostics GmbH, Mannheim, Germany) according to the following protocol: after heating for 10 min at 95°C, amplification was performed by 40 cycles of 3 s at 94°C, 5 s at 56°C and 20 s at 72°C, followed by a melting curve analysis. The fold induction of GS mRNA was calculated using the Relative Quantification Method of the Light Cycler 4.05 software (Roche Diagnostics GmbH).
Acknowledgments
We would like to thank D. Mahn, P. Metz, B. Proksch, C. Schulze and B. Woithe for excellent technical assistance. The HaCaT cells were generously provided by Prof. Fusenig (DKFZ Heidelberg, Germany). Part of the human skin samples were kindly provided by Dr. U. Anderegg (University of Leipzig, Germany).
Author Contributions
Conceived and designed the experiments: LD SZ RG GHB. Performed the experiments: LD SZ SS GVT JS AL GHB. Analyzed the data: LD SZ SS GVT DDR CHG RG GHB. Contributed reagents/materials/analysis tools: LD SZ DDR CHG RG. Wrote the paper: LD SZ RG GHB.
References
- 1. Chwals WJ (2004) Regulation of the cellular and physiological effects of glutamine. Med Chem 4: 833–838.
- 2. Lie-Venema H, de Boer PA, Moorman AF, Lamers WH (1997) Role of the 5′ enhancer of the glutamine synthetase gene in its organ-specific expression. Biochem J 323: 611–619.
- 3.
Gebhardt R, Mecke D (1984) Cellular distribution and regulation of glutamine synthetase in liver. In: Häussinger D, Sies H, editors. Glutamate metabolism in mammalian tissues. Heidelberg: Springer Verlag. pp. 98–121.
- 4. Gebhardt R, Gaunitz F, Mecke D (1994) Heterogeneous (positional) expression of hepatic glutamine synthetase: features, regulation and implications for hepatocarcinogenesis. Adv Enzyme Regul 34: 27–56.
- 5. Burch HB, Choi S, McCarthy WZ, Wong PY, Lowry OH (1978) The location of glutamine synthetase within the rat and rabbit nephron. Biochem Biophys Res Commun 82: 498–505.
- 6. Conjard A, Komaty O, Delage H, Boghossian M, Martin M, Ferrier B, Baverel G (2003) Inhibition of glutamine synthetase in the mouse kidney: a novel mechanism of adaptation to metabolic acidosis. J Biol Chem 278: 38159–38166.
- 7. Buniatian GH, Hartmann H-J, Traub P, Weser U, Wiesinger H, et al. (2001) Acquisition of blood-tissue barrier supporting features by hepatic stellate cells and astrocytes of myofibroblastic phenotype. Inverse dynamics of metallothionein and glial fibrillary acidic protein expression. Neurochem Int 38: 373–383.
- 8. Norenberg MD, Rao KV, Jayakumar AR (2005) Mechanisms of ammonia-induced astrocyte swelling. Metab Brain Dis 20: 303–318.
- 9. Bode JG, Peters-Regehr T, Gressner AM, Häussinger D (1998) De novo expression of glutamine synthetase during transformation of hepatic stellate cells into myofibroblast-like cells. Biochem J 335: 697–700.
- 10. Holash JA, Harik SI, Perry G, Stewart PA (1993) Barrier properties of testis microvessels. Proc Natl Acad Sci U S A 90: 11069–11073.
- 11. Plaitakis A, Shashidharan P (2000) Glutamate transport and metabolism in dopaminergic neurons of substantia nigra: implications for the pathogenesis of Parkinson's disease. J Neurol 247: S21125–21135.
- 12. Robinson SR (2000) Neuronal expression of glutamine synthetase in Alzheimer's disease indicates a profound impairment of metabolic interactions with astrocytes. Neurochem Int 36: 471–82.
- 13. Burbaeva GSh, Boksha IS, Tereshkina EB, Savushkina OK, Starodubtseva LI, et al. (2005) Glutamate metabolizing enzymes in prefrontal cortex of Alzheimer's disease patients. Neurochem Res 30: 1443–51.
- 14. Arola L, Palou A, Remesar X, Alemany M (1981) Changes in glutamine synthesis activity in the different organs of developing rats. Arch Int Physiol Biochim 89: 189–94.
- 15. Remesar X, Arola L, Palou A, Alemany M (1982) Glutamine synthetase activity in rat tissues during pregnancy and lactation. Horm metab Res 14: 419–21.
- 16. van Straaten HW, He Y, van Duist MM, Labruyere WT, Vermeulen JL, et al. (2006) Cllular concentrations of glutamine synthetase in murine organs. Biochem Cell Biol 84: 215–231.
- 17. Häberle J, Gorg B, Rutsch F, Schmidt E, Toutain A, et al. (2005) Congenital Glutamine Deficiency with Glutamine Synthetase Mutations. N Engl J Med 353: 1926–1933.
- 18. Häberle J, Görg B, Toutain A, Rutsch F, Benoist JF, et al. (2006) Inborn error of amino acid synthesis: Human glutamine synthetase dificiency. J Inherit Metab Dis 29: 352–358.
- 19. Abcouwer SF, Lohmann R, Bode BP, Lustig RJ, Souba WW (1997) Induction of glutamine synthetase expression after major burn injury is tissue specific and temporally variable. J Trauma 42: 421–427.
- 20. Ardawi MS (1988) Skeletal muscle glutamine production in thermally injured rats. Clin Sci (Lond) 74: 165–172.
- 21. Danielyan L, Tolstonog G, Traub P, Salvetter J, Gleiter CJ, et al. (2007) Colocalization of glial fibrillary acidic protein, metallothionein, and MHC II in human, rat, NOD/SCID, and nude mouse skin keratinocytes and fibroblasts. J Invest Dermatol 127: 555–563.
- 22. Le Prince G, Delaere P, Fages C, Lefrançois T, Touret M, et al. (1995) Glutamine synthetase (GS) expression is reduced in senile dementia of the Alzheimer type. Neurochem Res 20: 859–862.
- 23. Buniatian GH, Hartmann H-J, Traub P, Weser U, Wiesinger H, et al. (2001) Acquisition of blood-tissue barrier supporting features by hepatic stellate cells and astrocytes of myofibroblastic phenotype. Inverse dynamics of metallothionein and glial fibrillary acidic protein expression. Neurochem Int 38: 373–383.
- 24. Buniatian GH, Hartmann H-J, Traub P, Wiesinger H, Albinus M, et al. (2002) Glial fibrillary acidic protein-positive cells of the kidney are capable of raising a protective biochemical barrier similar to astrocytes: expression of metallothionein in podocytes. Anat Rec 267: 296–306.
- 25. Michel M, Török N, Godbout MJ, Lussier M, Gaudreau P, et al. (1996) Keratin 19 as a biochemical marker of skin stem cells in vivo and in vitro: keratin 19 expressing cells are differentially localized in function of anatomic sites, and their number varies with donor age and culture stage. J Cell Sci 109: 1017–1028.
- 26. Ya-Xian Z, Suetake T, Tagami H (1999) Number of cell layers of the stratum corneum in normal skin-relationship to the anatomical location on the body, age, sex and physical parameters. Arch Dermatol Res 291: 555–559.
- 27. Jablonski MM, Tombran-Tink J, Mrazek DA, Iannaccone A (2001) Pigment epithelium-derived factor supports normal Müller cell development and glutamine synthetase expression after removal of the retinal pigment epithelium. Glia 35: 14–25.
- 28. Seth A, Basuroy S, Sheth P, Rao RK (2004) L-Glutamine ameliorates acetaldehyde-induced increase in paracellular permeability in Caco-2 cell monolayer. Am J Physiol Gastrointest Liver Physiol 287: G510–517.
- 29. Li N, Lewis P, Samuelson D, Liboni K, Neu J (2004) Glutamine regulates Caco-2 cell tight junction proteins. Am J Physiol Gastrointest Liver Physiol 287: G726–733.
- 30. Padden M, Leech S, Craig B, Kirk J, Brankin B, McQuaid S (2007) Differences in expression of junctional adhesion molecule-A and beta-catenin in multiple sclerosis brain tissue: increasing evidence for the role of tight junction pathology. Acta Neuropathol 113: 177–186.
- 31. Gebhardt R, Baldysiak-Figiel A, Krugel V, Ueberham E, Gaunitz F (2007) Hepatocellular expression of glutamine synthetase: an indicator of morphogen actions as master regulators of zonation in adult liver. Prog Histochem Cytochem 41: 201–266.
- 32. Benhamouche S, Decaens T, Godard C, Chambrey R, Rickman DS, et al. (2006) Apc tumor suppressor gene is the “zonation-keeper” of mouse liver. Dev Cell 10: 759–770.
- 33. Boukamp P, Petrussevska RT, Breitkreutz D, Hornung J, Markham A, et al. (1988) Normal keratinization in a spontaneously immortalized aneuploid human keratinocyte cell line. J Cell Biol 106: 761–771.
- 34. Gebhardt R, Schrode W, Eisenmann-Tappe I (1998) Cellular characteristics of epithelial cell lines from juvenile rat liver: selective induction of glutamine synthetase by dexamethasone. Cell Biol Toxicol 14: 55–67.
- 35. Labow BI, Souba WW, Abcouwer SF (1999) Glutamine synthetase expression in muscle is regulated by transcriptional and posttranscriptional mechanisms. Am J Physiol 276: E1136–1145.
- 36. Chatauret N, Desjardins P, Zwingmann C, Rose C, Rao KV, et al. (2006) Direct molecular and spectroscopic evidence for increased ammonia removal capacity of skeletal muscle in acute liver failure. J Hepatol 44: 1083–1088.
- 37. Stambolic V, Ruel L, Woodgett JR (1996) Lithium inhibits glycogen synthase kinase-3-ß activity and mimics wingless signalling in intact cells. Curr Biol 6: 1664–1668.
- 38. Kruithof-de Julio M, Labruyère WT, Ruijter JM, Vermeulen JLM, Stanulovic V, et al. (2005) The RL-ET-14 cell line mediates expression of glutamine synthetase through the upstream enhancer/promoter region. J Hepatol 43: 126–131.
- 39. Elias PM (2005) Stratum corneum defensive functions: an integrated view. J Invest Dermatol 125: 183–200.
- 40. Malminen M, Koivukangas V, Peltonen J, Karvonen SL, Oikarinen A, et al. (2003) Immunohistological distribution of the tight junction components ZO-1 and occludin in regenerating human epidermis. Br J Dermatol 149: 255–260.
- 41. Troy TC, Turksen K (2007) The targeted overexpression of a Claudin mutant in the epidermis of transgenic mice elicits striking epidermal and hair follicle abnormalities. Mol Biotechnol 36: 166–174.
- 42. Eckert RL, Green H (1986) Structure and evolution of the human involucrin gene. Cell 46: 583–589.
- 43. Marshall D, Hardman MJ, Nield KM, Byrne C (2001) Differentially expressed late constituents of the epidermal cornified envelope. Proc Natl Acad Sci U S A 98: 13031–13036.
- 44. Yoneda K, McBride OW, Korge BP, Kim IG, Steinert PM (1992) The cornified cell envelope: loricrin and transglutaminases. J Dermatol 19: 761–764.
- 45. Sevilla LM, Nachat R, Groot KR, Klement JF, Uitto J, et al. (2007) Mice deficient in involucrin, envoplakin, and periplakin have a defective epidermal barrier. J Cell Biol 179: 1599–1612.
- 46. Pummi K, Malminen M, Aho H, Karvonen SL, Peltonen J, et al. (2001) Epidermal tight junctions: ZO-1 and occludin are expressed in mature, developing, and affected skin and in vitro differentiating keratinocytes. J Invest Dermatol 117: 1050–1058.
- 47. Chakraborty T, Chatterjee A, Rana A, Srivastawa S, Damodaran S, et al. (2007) Cell proliferation and hepatocarcinogenesis in rat initiated by diethylnitrosamine and promoted by phenobarbital: potential roles of early DNA damage and liver metallothionein expression. Life Sci 81: 489–99.
- 48. Penkowa M, Hidalgo J (2000) Metallothionein I+II expression and their role in experimental autoimmune encephalomyelitis. Glia 32: 247–263.
- 49. Mirlean N, Roisenberg A (2006) The effect of emissions of fertilizer production on the environment contamination by cadmium and arsenic in southern Brazil. Environ Pollut 143: 335–340.
- 50. Prozialeck WC, Wellington DR, Lamar PC (1993) Comparison of the cytotoxic effects of cadmium chloride and cadmium-metallothionein in LLC-PK1 cells. Life Sci 53: PL337–342.
- 51. Wong CH, Mruk DD, Lui WY, Cheng CY (2004) Regulation of blood-testis barrier dynamics: an in vivo study. J Cell Sci 117: 783–798.
- 52. Gebhardt R, Reichen J (1994) Changes in distribution and activity of glutamine synthetase in carbon tetrachloride-induced cirrhosis in the rat: potential role in hyperammonemia. Hepatology 20: 684–691.
- 53. Han EK, Guadagno TM, Dalton SL, Assoian RK (1993) A cell cycle and mutational analysis of anchorage-independent growth: cell adhesion and TGF-beta 1 control G1/S transit specifically. J Cell Biol 122: 461–471.
- 54. Filipe JA, Nunes JP (2002) Functional importance of the actin cytoskeleton in contraction of bovine iris sphincter muscle. Auton Autacoid Pharmacol 22: 155–159.
- 55. Kubler MD, Watt FM (1993) Changes in the distribution of actin-associated proteins during epidermal wound healing. J Invest Dermatol 100: 785–789.
- 56. Zhang L, Deng M, Parthasarathy R, Wang L, Mongan M, et al. (2005) MEKK1 transduces activin signals in keratinocytes to induce actin stress fiber formation and migration. Mol Cell Biol 25: 60–65.
- 57. Braga VM, Hodivala KJ, Watt FM (1995) Calcium-induced changes in distribution and solubility of cadherins, integrins and their associated cytoplasmic proteins in human keratinocytes. Cell Adhes Commun 3: 201–215.
- 58. Hartsock A, Nelson WJ (2008) Adherens and tight junctions: Basic structure, function and connections to the actin cytoskeleton. Biochim Biophys Acta 1778: 660–669.
- 59. Ivanov AI, Bachar M, Babbin BA, Adelstein RS, Nusrat A, Parkos CA (2007) A unique role for nonmuscle myosin heavy chain IIA in regulation of epithelial apical junctions. PLoS ONE 2: e658.
- 60. Zhu Q, Emanuele NV, Van Thiel DH (2004) Calponin is expressed by Sertoli cells within rat testes and is associated with actin-enriched cytoskeleton. Cell Tissue Res 316: 243–253.
- 61. Hasan W, Zhang R, Liu M, Warn JD, Smith PG (2000) Coordinate expression of NGF andalpha-smooth muscle actin mRNA and protein in cutaneous wound tissue ofdeveloping and adult rats. Cell Tissue Res 300: 97–109.
- 62. Buniatian GH (2003) Stages of activation of hepatic stellate cells (HSC): effects of ellagic acid, an inhibiter of liver fibrosis, on the antigenic and morphologic differentiation of cultured HSC. Cell Proliferat 38: 307–319.
- 63. Fischer H, Eckhart L, Mildner M, Jaeger K, Buchberger M, et al. (2007) DNase1L2 degrades nuclear DNA during corneocyte formation. J Invest Dermatol 127: 24–30.
- 64. Houben E, De Paepe K, Rogiers V (2007) A Keratinocyte's cours of life. Skin Pharmacol Physiol 20: 122–132.
- 65. Jensen JM, Förl M, Winoto-Morbach S, Seite S, Schunck M, et al. (2005) Acid and neutral sphingomyelinase, ceramide synthase, and acid ceramidase activities in cutaneous aging. Exp Dermatol 14: 609–618.
- 66. Pinel C, Coxam V, Mignon M, Taillandier D, Cubizolles C, et al. (2006) Alterations in glutamine synthetase activity in rat skeletal muscle are associated with advanced age. Nutrition 22: 778–785.
- 67. Niemann C (2006) Controlling the stem cell niche: right time, right place, right strength. Bioessays 28: 1–5.
- 68. Dénes Z (1985) Age and the neck's “décolleté syndrome”. The neck is an age sensitive region of the skin. ZFA 40: 159–164.
- 69. Desjardins P, Rao KV, Michalak A, Rose C, Butterworth RF (1999) Effect of portacaval anastomosis on glutamine synthetase protein and gene expression in brain, liver and skeletal muscle. Metabolic Brain Disease 14: 273–280.
- 70. Eizayaga F, Scorticati C, Prestifilippo JP, Romay S, Fernandez MA, et al. (2006) Altered blood-brain barrier permeability in rats with prehepatic portal hypertension turns to normal when portal pressure is lowered. World J Gastroenterol 12: 1367–1372.
- 71. Keiding S, Sørensen M, Bender D, Munk OL, Ott P, et al. (2006) Brain metabolism of 13N-ammonia during acute hepatic encephalopathy in cirrhosis measured by positron emission tomography. Hepatology 43: 42–50.
- 72. Suárez I, Bodega G, Fernández B (2002) Glutamine synthetase in brain: effect of ammonia. Neurochem Int 41: 123–142.
- 73. Olde Damink SW, Jalan R, Redhead DN, Hayes PC, Deutz NE, et al. (2002) Interorgan ammonia and amino acid metabolism in metabolically stable patients with cirrhosis and a TIPSS. Hepatology 36: 1163–1171.
- 74. Girard G, Butterworth RF (1992) Effect of portacaval anastomosis on glutamine synthetase activities in liver, brain, and skeletal muscle. Dig Dis Sci 37: 1121–1126.
- 75. Dejong CH, Deutz NE, Soeters PB (1994) Muscle ammonia and glutamine exchange during chronic liver insufficiency in the rat. J Hepatol 21: 299–307.
- 76. Nose K, Mizuno T, Yamane N, Kondo T, Ohtani H, et al. (2005) Identification of ammonia in gas emanated from human skin and its correlation with that in blood. Anal Sci 21: 1471–1474.
- 77. Leyden JJ, Katz S, Stewart R, Kligman AM (1977) Urinary ammonia and ammonia-producing microorganisms in infants with and without diaper dermatitis. Arch Dermatol 113: 1678–1680.
- 78. Ziylan YZ, Uzüm G, Bernard G, Diler AS, Bourre JM (1993) Changes in the permeability of the blood-brain barrier in acute hyperammonemia. Effect of dexamethasone. Mol Chem Neuropathol 20: 203–218.
- 79. Vastag M, Neuhofer W, Nagel W, Beck FX (2005) Ammonium affects tight junctions and the cytoskeleton in MDCK cells. Pflugers Arch 449: 384–391.
- 80. Sullivan DM, Jensen TG, Taichman LB, Csaky KG (1997) Ornithine-delta- aminotransferase expression and ornithine metabolism in cultured epidermal keratinocytes: toward metabolic sink therapy for gyrate atrophy. Gene Therapy 4: 1036–1044.
- 81. Hansson E (1989) Regulation of glutamine synthetase synthesis and activity by glucocorticoids and adrenoceptor activation in astroglial cells. Neurochem Res 14: 585–587.
- 82. O'Banion MK, Young DA, Bohn MC (1994) Corticosterone-responsive mRNAs in primary rat astrocytes. Brain Res Mol Brain Res 22: 57–68.
- 83. Abcouwer SF, Bode BP, Souba WW (1995) Glucocorticoids regulate glutamine synthetase expression in a tissue-specific manner. J Surg Res 59: 59–65.
- 84. Jackson MJ, Zielke HR, Max SR (1995) Effect of dibutyryl cyclic AMP and dexamethasone on glutamine synthetase gene expression in rat astrocytes in culture. Neurochem Res 20: 201–207.
- 85. Patel AJ, Hunt A (1985) Observations on cell growth and regulation of glutamine synthetase by dexamethasone in primary cultures of forebrain and cerebellar astrocytes. Brain Res 350: 175–184.
- 86. Soni T, Wolfrom C, Guerroui S, Raynaud N, Poggi J, et al. (1991) Respective effects of glucose and glutamine on the glutamine synthetase activity of human skin fibroblasts. Mol Cell Biochem 102: 149–154.
- 87. Jaenicke L, Berson W (1977) Glutamine synthetase from pig brain: Binding of adenosine thiphosphate. Hoppe-Seyler's Z Physiol Chem 358: 883–889.
- 88.
Zellmer S, Reissig D (2001) Isolation, cultivation and differentiation of normal human keratinocytes in serum-free medium. In: Wise C, editor. Epithelial cell culture protocols,. Totowa, New Jersey: Humana Press Inc.. pp. 179–184.
- 89. Bayreuther K, Francz PI, Gogol J, Kontermann K (1992) Terminal differentiation, aging, apoptosis, and spontaneous transformation in fibroblast stem cell systems in vivo and in vitro. Ann N Y Acad Sci 663: 167–179.
- 90. Hamprecht B, Löffler F (1985) Primary glial cultures as a model for studying hormonal action. Methods Enzymol 109: 341–345.
- 91. Buniatian G, Gebhardt R, Schrenk D, Hamprecht B (1996) Colocalization of three types of intermediate filament proteins in perisinusoidal stellate cells: glial fibrillary acidic protein as a new cellular marker. Eur J Cell Biol 70: 23–32.
- 92. Nagel W, Hartmann H-J, Weser U (1990) Monoclonal antibodies to monomeric rat liver metallothionein-I: the immunoreactivity of lysine residues in metallothionein. Immunol Lett 26: 291–295.
- 93. Levintow L (1954) The glutamyltransferase activity of normal and neoplastic tissues. J Natl Cancer Inst 15: 347–352.
- 94. Gebhardt R, Williams GM (1986) Amino acid transport in established adult rat liver epithelial cell lines. Cell Biol Toxicol 2: 9–20.
- 95. Bradford MM (1976) A rapid and sensitive method for the quantitation of microgram quantities of protein utilizing the principle of protein-dye binding. Anal Biochem 72: 248–254.