Liver Biology and Pathobiology...Pathobiology
Mechanism of action of the antifibrogenic compound gliotoxin in rat liver cells
Article first published online: 30 JUN 2004
Copyright © 2004 American Association for the Study of Liver Diseases
Volume 40, Issue 1, pages 232–242, July 2004
How to Cite
Orr, J. G., Leel, V., Cameron, G. A., Marek, C. J., Haughton, E. L., Elrick, L. J., Trim, J. E., Hawksworth, G. M., Halestrap, A. P. and Wright, M. C. (2004), Mechanism of action of the antifibrogenic compound gliotoxin in rat liver cells. Hepatology, 40: 232–242. doi: 10.1002/hep.20254
- Issue published online: 30 JUN 2004
- Article first published online: 30 JUN 2004
- Manuscript Accepted: 21 MAR 2004
- Manuscript Received: 26 JUN 2003
- Biotechnology and Biological Sciences Research Council Ph.D. and Ph.D. (CASE) studentships
- Scottish Hospitals Endowment Research Trust
Gliotoxin has been shown to promote a reversal of liver fibrosis in an animal model of the disease although its mechanism of action in the liver is poorly defined. The effects of gliotoxin on activated hepatic stellate cells (HSCs) and hepatocytes have therefore been examined. Addition of gliotoxin (1.5 μM) to culture-activated HSCs resulted in its rapid accumulation, resulting in increased levels of glutathione and apoptosis without any evidence of oxidative stress. In contrast, although hepatocytes also rapidly sequestered gliotoxin, cell death only occurred at high (50-μM) concentrations of gliotoxin and by necrosis. At high concentrations, gliotoxin was metabolized by hepatocytes to a reduced (dithiol) metabolite and glutathione was rapidly oxidized. Fluorescent dye loading experiments showed that gliotoxin caused oxidative stress in hepatocytes. Antioxidants—but not thiol redox active compounds—inhibited both oxidative stress and necrosis in hepatocytes. In contrast, HSC apoptosis was not affected by antioxidants but was potently abrogated by thiol redox active compounds. The adenine nucleotide transporter (ANT) is implicated in mitochondrial-dependent apoptosis. HSCs expressed predominantly nonliver ANT isoform 1, and gliotoxin treatment resulted in a thiol redox-dependent alteration in ANT mobility in HSC extracts, but not hepatocyte extracts. In conclusion, these data suggest that gliotoxin stimulates the apoptosis of HSCs through a specific thiol redox-dependent interaction with the ANT. Further understanding of this mechanism of cell death will aid in finding therapeutics that specifically stimulate HSC apoptosis in the liver, a promising approach to antifibrotic therapy. Supplementary material for this article can be found on the HEPATOLOGY website (http://interscience.wiley.com/jpages/0270-9139/suppmat/index.html). (HEPATOLOGY 2004;40:232–242.)
A common outcome in patients with chronic liver damage is the development of scarring fibrosis, a wound-healing response that is primarily associated with the production of extracellular matrix protein by hepatic stellate cells (HSCs).1, 2 HSCs in normal liver are in relative low abundance, reside in the space of Disse, and function to store vitamin A in the form of fatty acid esters.3 Chronic liver damage results in HSC transdifferentiation from the “quiescent” vitamin A–storing to an “activated” myofibroblast-like (α-smooth muscle actin-expressing) phenotype.1, 2 HSC activation results in their proliferation and up-regulation in the expression of genes contributing to matrix accumulation such as collagen type I and tissue inhibitors of metalloproteinases.4
Increasing evidence suggests that rats recover from liver fibrosis through up-regulation of apoptosis of activated HSC.5–8 The epipolythiodioxopiperazine fungal metabolite gliotoxin kills rat and human HSCs by stimulating their apoptosis; administration of gliotoxin to rats (treated with either carbon tetrachloride or thioacetamide to cause liver fibrosis) significantly reduced the number of activated HSCs in the liver and the extent of scarring fibrosis.5, 9 An up-regulation of the apoptosis of activated HSC may be an effective therapeutic approach to treat liver fibrosis.
Nuclear factor κB (NF-κB) is a transcription factor that regulates cell proliferation and apoptosis in addition to immune and inflammatory responses.10 In most cells, including “unstimulated” hepatocytes, NF-κB is inactive (under normal conditions it is bound to inhibitory I-κB proteins that mask a nuclear localization signal) and retained in the cytosol.10, 11 Cytokines such as tumor necrosis factor α (TNF-α)—which are known to play a role in liver fibrogenesis1, 2—activate NF-κB in hepatocytes by stimulating a degradation of the I-κB protein.10 Through the same receptor, TNF-α also activates an apoptotic pathway that involves the opening of a pore in mitochondria (termed the mitochondrial permeability transition [MPT]) resulting in cytochrome c release, activation of caspases and apoptosis.12 The parallel activation of NF-κB by TNF-α appears to prevent hepatocyte apoptosis through induction of antiapoptotic gene expression because an inhibition of NF-κB-dependent gene expression (using either a general inhibitor of gene expression or by specifically inhibiting NF-κB activation) results in hepatocyte apoptosis.12–15 Accordingly, in vivo, TNF-α stimulates hepatocyte proliferation/liver regeneration16—an essential response to liver insult. Gliotoxin, as an inhibitor of NF-κB activation through its inhibition of I-κB degradation, therefore diverts hepatocytes to undergo apoptosis when also treated with TNF-α.13 In culture-activated (i.e., α-smooth muscle actin-expressing) HSCs, NF-κB is constitutively active, and gliotoxin stimulates the apoptosis of HSCs without the need for the addition of cytokines such as TNF-α.5, 17 However, we have shown that gliotoxin only inhibits TNF-α–inducible NF-κB DNA binding activity in activated HSCs and not constitutively-activated NF-κB.5 Indeed, other inhibitors of NF-κB activation, such as calpain inhibitor I, did not stimulate activated HSC apoptosis.5
The hypothesis underpinning these experiments is that NF-κB is not involved in gliotoxin-dependent activated HSC killing (in the absence of TNF-α), and that there may be an NF-κB-independent pathway of gliotoxin-stimulated HSC apoptosis in addition to an NF-κB–dependent pathway. One potential target for gliotoxin may be the adenine nucleotide transporter (ANT), a protein located on the inner mitochondrial membrane that functions to carry adenosine diphosphate and adenosine triphosphate across the membrane. In combination with cyclophilin D, the voltage-depedent anion channel, and several kinases, the ANT regulates inner membrane permeability to low molecular weight compounds referred to as the MPT.18 The MPT is an important determinant in cell death that, under certain conditions, results in cytochrome c release from the mitochondrial membrane space, caspase activation, and apoptosis.18
A detailed examination of the effects of gliotoxin on liver cells (hepatocytes and HSCs) has been examined, because gliotoxin or a related compound could prove useful in the treatment of liver fibrosis.19
Materials and Methods
Animals, Cell Isolation, and Culture.
Male Sprague-Dawley rats (250–300 g) were bred in house at the Biological Services Unit, Foresterhill, University of Aberdeen, UK. Rat hepatocytes were prepared by collagenase perfusion essentially as described previously.20 Hepatocytes were cultured in William's Medium E supplemented with 1 μg/mL of bovine insulin, 10% fetal calf serum, 80 U/mL of penicillin, and 80 μg/mL of streptomycin on collagen type I–coated plates (BD Biosciences, Oxford, UK). Rat HSCs were isolated through pronase/collagenase perfusion of the liver followed by density gradient centrifugation as described previously.5 HSCs were cultured in Dulbecco's Modified Eagle Medium containing 4.5 g/L of glucose, supplemented with 16% (v/v) fetal calf serum, 80 U/mL of penicillin, 80 μg/mL of streptomycin, and 32 μg/mL of gentamicin. Cells were seeded onto plastic culture dishes, under which conditions the cells became activated as evidenced by the expression of α-smooth muscle actin.1, 2 HSCs were used within the first two passages.
All cells were incubated at 37°C in a humidified incubator gassed with 5% CO2 in air. Hepatocytes were maintained in William's Medium E optimally, whereas HSCs were widely cultured in Dulbecco's Modified Eagle Medium. Experiments were therefore performed with cells in their respective optimal media. The effects of gliotoxin were not significantly affected by the type of culture medium employed for the two cell types in that the effects of gliotoxin on each cell type was also observed if incubations were performed in the alternative medium (data not shown).
Assessments of Cell Viability and Apoptosis.
Cell attachment was assessed by visual examination of the cells. The ability of cells to exclude the dye trypan blue was examined by the addition of trypan blue to give a final concentration of 0.05% (w/v).21 Caspase 3 (DEVDase) activity was determined using a colorimetric CaspACE kit (Promega, Southampton, UK) according to the manufacturer's instructions. Total protein was determined by the method of Bradford.22 4′,6′-Diamidino-2-phenylindole was used to stain DNA in formalin-fixed cells for the analysis of nuclear changes in response to various treatments.
Determination of Cellular Glutathione Levels.
Cellular reduced glutathione (GSH) and oxidized glutathione (GSSG) levels were determined essentially as previously described.23 The concentrations of GSH and GSSG were determined via peak integration using authentic standards.
Metabolism of Gliotoxin.
The medium was removed and cells were washed with HEPES/HBSS buffer (0.14 M NaCl, 5.4 mM KCl, 0.34 mM Na2HPO4, 0.44 mM KH2PO4, 5.6 mM glucose, 1 mM CaCl2, 6 mM HEPES, 4 mM NaHCO3 pH 7.4) and incubated with gliotoxin in 1.5 mL of HEPES/HBSS buffer per well of a six-well plate. The levels of gliotoxin were determined using high performance liquid chromatography (HPLC; Sollentuna, Sweden) essentially as outlined previously24 through direct injection of medium samples onto a Gilson HPLC machine fitted with a 10-cm Hichrom C18 reverse phase column (Theale, UK) (internal diameter: 4.6 mm).
2′,7′-Dichlorodihydrofluorescein Diacetate Detection of Reactive Oxygen Species.
Hepatocytes and HSCs were loaded with 2′,7′-dichlorodihydrofluorescein diacetate (H2DCFDA) and viewed under a confocal microscope to visualize reactive oxygen species (ROS) using a variation of a method described previously.25 Cells in a six-well plate were dosed with 10 μM H2DCFDA and incubated at 37°C for 20 minutes. Medium was removed and replaced with 3 mL of HEPES/HBSS buffer to which the required treatment was added. Cells were incubated for a further 20 minutes at 37°C. Cells were then examined using a confocal microscope using a ×20 objective at an excitation wavelength of 488 nm. Emission between 530–560 nm was detected and analyzed using Biorad Lasersharp software (Hemel Hempstead, UK).
Western blotting was performed essentially as outlined previously,26 except that in some cases (indicated in legends) the reducing agent (dithiothreitol) was omitted during SDS detergent denaturation of samples. A rabbit polyclonal antiserum to rat ANT was prepared as previously described.27 Detection was achieved using an ECL kit (Amersham, UK).
Student's t test (two-tailed) was used to test for replicate statistical significance from one experiment and was typical of the number of separate experiments reported in the figure legends. Results were consistently observed to be statistically significant in all other experiments.
The Toxicity of Gliotoxin in Liver Cells In Vitro.
Hepatocytes and HSCs were prepared from rat liver and cultured separately as outlined in Materials and Methods. Fig. 1A demonstrates that concentrations in excess of 10 μM of gliotoxin resulted in hepatocyte detachment (typically a concentration of between 30 and 50 μM of gliotoxin was required for extensive detachment of hepatocytes), whereas 1.5 μM of gliotoxin (a concentration without any apparent effect in hepatocytes) resulted in almost complete detachment of HSCs within 3 hours. Both hepatocytes and HSCs were equally sensitive to chlorpromazine (a Ca2+/calmodulin antagonist that causes mitochondrial dysfunction at concentrations above 150 μM),28 whereas microcystin—an agent known to cause hepatocyte apoptosis29, 30—specifically stimulated the detachment of hepatocytes (see Fig. 1).
The mechanism of exclusion of trypan blue dye from cells is not fully understood, but we do know that it relies on an energy-dependent process.21, 31 Because apoptosis is an energy-dependent (often programmed) event, cells that undergo apoptosis exclude trypan blue for a period, despite the morphological appearance of death.31 Fig. 2A and 2C demonstrate that toxic (50 μM) concentrations of gliotoxin (i.e., a concentration that resulted in detachment from the substratum) gave rise to hepatocytes that did not exclude trypan blue. This is similar to the effects seen with 200 μM chlorpromazine but not with agents that cause hepatocyte apoptosis (i.e., 100 nM microcystin [see Fig. 2A and 2C]) or TNF-α together with the protein synthesis inhibitor cycloheximide12 (see Fig. 2C). In contrast, concentrations of gliotoxin above 1.5 μM that caused activated HSC detachment from the substratum resulted in HSCs that retained the ability to exclude trypan blue, whereas chlorpromazine treatment resulted in HSCs that were unable to exclude trypan blue (Fig. 2B and 2C). Fig. 2B also shows that gliotoxin treatment of HSCs resulted in the cleavage of DNA to a nucleosomal ladder as previously reported.5
Caspase 3 is a protease known to function as a distal executioner of many apoptotic programs.32 Fig. 3 indicates that hepatocytes treated with gliotoxin—including concentrations that caused substratum detachment—did not contain increased levels of caspase 3 activity similar to cells treated with chlorpromazine. In contrast, treatment with TNF-α/cycloheximide or microcystin alone—treatments known to stimulate hepatocyte apoptosis12, 29—resulted in significant increases in caspase 3 activity (see Fig. 3). In contrast to hepatocytes, HSCs treated with gliotoxin showed a dose-dependent significant increase in caspase 3 activity (see Fig. 3). Compounds that either had no effect in HSCs (microcystin) or caused HSC necrosis (chlorpromazine) did not result in an increase in caspase 3 activity (see Fig 3).
Nuclear changes are diagnostic of regulated apoptotic mechanisms of cell death.32 Supplementary Fig. 1 shows that toxic levels of gliotoxin did not stimulate hepatocyte nuclear condensation as observed when hepatocytes were treated with known proapoptotic TNF-α/cycloheximide agents in contrast to both gliotoxin and TNF-α/cycloheximide treatments in activated HSCs.
These data show that activated HSCs were significantly more sensitive to the toxic effects of gliotoxin than hepatocytes and that gliotoxin stimulated an apoptotic mechanism of cell death in HSCs. In contrast, concentrations of gliotoxin toxic to hepatocytes resulted in unambiguous necrosis. It should be noted, however, that a proportion of hepatocytes treated with gliotoxin soon after their isolation (0–2 hours) underwent apoptosis (data not shown) likely associated with an inhibition by gliotoxin of NF-κB activity (which is briefly activated in response to hepatocyte isolation33).
The Uptake and Metabolism of Gliotoxin by Hepatocytes and HSCs.
To determine the underlying causes of the differential effects of gliotoxin in hepatocytes and HSCs, gliotoxin uptake and metabolism were examined in pure hepatocyte and activated HSCs cultures. Supplementary Fig. 2A indicates that both hepatocytes and activated HSCs rapidly removed gliotoxin from the culture medium in a time-dependent fashion. HSCs sequestered approximately 1.5 times as much gliotoxin per unit of protein than hepatocytes; however, the increased levels sequestered by HSCs could not account for the difference in the mode of cell death between hepatocytes and HSCs.
Supplementary Fig. 2B and 2C indicate that gliotoxin was metabolized to several different metabolites. Metabolite A had a retention time identical with dithiothreitol (DTT)-reduced or GSH-reduced gliotoxin (Supplementary Fig. 3B), suggesting that this metabolite is reduced dithiol gliotoxin. Metabolites B–D have been shown to be gliotoxin-glutathione conjugates.34 Metabolite E is unidentified. These metabolites were not produced by activated HSCs at 10 μM gliotoxin concentrations or below. At high (50 μM) concentrations of gliotoxin and after 120 minutes of incubation, reduced dithiol gliotoxin (metabolite A) and very low levels of a glutathione conjugate (metabolite B) were detected (see Supplementary Fig. 2B). These data suggest that metabolism of gliotoxin by HSC is not required for the stimulation of HSC apoptosis since apoptosis occurs in the absence of any apparent metabolite production. In contrast, the more rapid and extensive metabolism of gliotoxin by hepatocytes may be associated with either the avoidance of apoptosis and/or results in their necrosis.
The Effect of Gliotoxin on the Levels of Glutathione in Hepatocytes and HSCs.
Because gliotoxin contains a dithiol bridge that is neccesary for the proapoptotic effects of this compound in HSCs,5, 35–37 the effect of gliotoxin on the levels of glutathione in hepatocytes and activated HSCs was examined. Supplementary Fig. 3A indicates that the addition of gliotoxin to GSH in (a cell-free) HEPES/HBSS buffer system resulted in direct oxidation of GSH to GSSG, suggesting that there is potential for a direct reaction of gliotoxin with GSH (and other thiols) in cells. Supplementary Fig. 3B confirms that there was a conversion of gliotoxin to reduced dithiol gliotoxin by GSH or by DTT. The decrease in detectable (derivatized) GSH in this cell-free system could not be accounted for through oxidation alone, suggesting that GSH directly reacts with gliotoxin to form conjugates. However, although a gliotoxin-GSH conjugate would still be expected to be derivatizable, conjugates (such as metabolites B, C, or D seen with hepatocytes [see Supplementary Fig. 2B]) were not detected by this HPLC assay (not shown) or the gliotoxin HPLC assay (see Supplementary Fig 3B). Supplementary Fig. 3C indicates that the addition of 50 μM of gliotoxin (levels that cause hepatocyte necrosis) to rat hepatocytes resulted in a rapid and sustained depletion of GSH to approximately 30%–40% of control levels by 3 hours (Supplementary Fig. 3E) with detectable increases in GSSG levels—at least during earlier timepoints (see Supplementary Fig. 3C). This depletion of glutathione in hepatocytes was also observed when cells were treated with 200 μM of chlorpromazine or 1 mM N-ethylmaleimide (Supplementary Fig. 3E), compounds which also caused hepatocyte necrosis (see Figs. 1 and 2). In contrast, treatments that caused hepatocyte apoptosis (TNF-α plus cycloheximide or microcystin) did not result in a depletion of cellular glutathione (see Supplementary Fig. 3E). Subhepatocyte toxic 1.5 μM gliotoxin resulted in an increase in glutathione levels (see Supplementary Fig. 3E).
Supplementary Figure 3D and E indicate that a concentration of 1.5 μM of gliotoxin—a concentration that caused the complete apoptosis of activated HSCs—resulted in a significant increase in activated HSC GSH levels as also observed with TNF-α/cycloheximide treatment. Chlorpromazine results in a significant reduction in GSH levels and, along with the sulfhydryl reagent N-ethylmaleimide, caused cell death by necrosis (see Supplementary Fig. 3). In all treatments, however, there was no detectable generation of GSSG in HSCs.
ROS Generation as a Mechanism of Necrotic Cell Death in Hepatocytes Exposed to Gliotoxin.
GSH oxidation in cell-free systems and reductions in hepatocyte GSH levels in hepatocytes (with a transient increase in GSSG levels) suggests that gliotoxin may alter the redox status of cells and promote oxidative stress. Reduction of gliotoxin as observed in a cell-free system and in hepatocytes in these studies (see Supplementary Figs. 2B and 2C and 3B) could initiate a cycle of gliotoxin reduction and oxidation (redox cycling) that may generate superoxide and other ROS. Hepatocytes and activated HSCs were therefore loaded with a cell-permeable dye (H2DCFDA) that, when de-esterified in cells, is fluorescent under oxidative conditions.38 Figure 4A indicates that hepatocytes loaded with H2DCFDA fluoresced significantly after treatment with gliotoxin, particularly at 7.5-μM and 50-μM concentrations. In contrast, activated HSCs under the same treatment and optical conditions did not fluoresce significantly (see Fig. 4A). To confirm that a lack of fluorescence from gliotoxin-treated HSCs is not associated with different optical settings or treatment conditions, fluorescence was examined in H2DCFDA-loaded hepatocyte/HSC cocultures. Fig. 4B indicates that fluorescence was almost exclusively limited to hepatocytes. Because the apparent lack of fluorescence in gliotoxin-treated HSC may be associated with either a lack of uptake and/or de-esterification of H2DCFDA, hepatocyte and HSC extracts were incubated with H2DCFDA, and the level of fluorescence was examined after the addition of pro-oxidant (H2O2 and FeCl2; gliotoxin and GSH). Fig. 4C shows that H2DCFDA was not fluorescent in the absence of cell extract addition, even in the presence of pro-oxidants. Addition of either hepatocyte or HSC extract led to the production of fluorescence upon the addition of pro-oxidants, suggesting that both hepatocytes and HSCs are able to de-esterify H2DCFDA to a product that is fluorescent in the presence of oxidative conditions. However, the levels of fluorescence from H2DCFDA de-esterified by HSC extracts were lower than the levels of fluorescence from H2DCFDA de-esterifed by hepatocyte extracts. HSCs may therefore have a lower capacity for de-esterifying H2DCFDA, which may modulate the levels of fluorescence emitted by HSCs. To test this possibility, H2DCFDA-loaded hepatocyte and HSCs were treated with H2O2 and FeCl2. Fig. 4D indicates that both hepatocytes and HSCs significantly fluoresced after treatment with H2O2 and FeCl2. HSCs are therefore able to sequester and de-esterify H2DCFDA. The lack of fluorescence in HSCs treated with gliotoxin is therefore likely to be due to a significantly lower production of ROS in HSCs compared with hepatocytes.
The Effect of Thiol Reducing Agents and Antioxidants on the Toxicity of Gliotoxin in Hepatocytes and Activated HSCs.
The structure of gliotoxin (Supplementary Fig. 4) includes a dithiol bridge, and Supplementary Fig. 3B indicates that this compound is susceptible to reduction by cellular-reduced thiols such as GSH, even in cell-free systems. Fig. 5A indicates that apoptosis of activated HSCs was potently blocked by the thiol-reducing agent DTT but also by the thiol-active agent pyrrolidine dithiocarbamate (PDTC). In contrast, hepatocyte cell death in response to gliotoxin was unaffected or potentiated by the addition of DTT and PDTC, respectively. Other compounds that block the nucleosomal ladder formation in HSCs after treatment with gliotoxin (Quin2-AM and caspase inhibitor 1)5 also had no effect on gliotoxin toxicity in hepatocytes. In contrast, the antioxidant catalase significantly reduced gliotoxin toxicity in hepatocytes, whereas addition to gliotoxin-treated HSCs had no effect (see Fig. 5A). Note that in these experiments (Fig. 5), the mode of cell death for HSCs (apoptosis) and hepatocytes (necrosis) was not altered by the addition of other compounds as judged by trypan blue exclusion (data not included). The addition of several components to reduce the levels of ROS in HSC cultures was without any detectable effect on gliotoxin-dependent HSC apoptosis, whereas the addition of catalase and superoxide dismutase (SOD) was the most potent abbrogator of hepatocyte necrosis (see Fig. 5A). The addition of catalase and SOD significantly reduced the levels of ROS detectable in H2DCFDA-loaded hepatocytes (Fig. 5B), supporting the suggestion that ROS generation is the mechanism of cell death in hepatocytes treated with gliotoxin. A major component of the complex of proteins that regulate the MPT is ANT. Figure 6A demonstrates that there is a different expression profile of the ANT isoforms between HSCs and hepatocytes as determined by Western blotting, with HSCs expressing predominantly ANT1 (cardiac/skeletal muscle isoform), whereas hepatocytes express the ANT2 isoform (although culture conditions appear to result in the expression of ANT1 isoform). To determine if the specific effects of gliotoxin in HSCs is associated with the ANT, HSCs and hepatocytes were treated with gliotoxin, PDTC and/or DTT and the migration of ANT under denaturing but nonreducing gel conditions examined. Figure 6B demonstrates that the ANT1 isoform in HSCs had variable redox status under nonreducing gel conditions, because at least two distinct bands are observed. Treatment with 1.5 μM of gliotoxin to cause HSC apoptosis resulted in an alteration in the migration of the slower migrating HSC ANT band that was prevented by addition to the culture medium of either PDTC or DTT. Treatment with 50 μM of gliotoxin resulted in an apparent loss of ANT—although under nonreducing gel conditions this could be caused by an oligomerization of proteins to high molecular weight complexes that did not enter the gel. Interestingly, PDTC promotes the formation of the ANT dimer in HSCs, but neither PDTC nor DTT caused cell death in HSCs in the short term. Under nonreducing gel conditions, hepatocyte ANT isoforms migrated as a single band, and gliotoxin treatment did not result in detectable alteration in ANT migration (Fig. 6C).
Our data demonstrate markedly altered effects of gliotoxin on different cell types of the liver. The mechanism of hepatocyte death is likely to be dependent on gliotoxin metabolism because hepatocytes rapidly generated several metabolites of gliotoxin that were not generated in HSCs. In view of gliotoxin's interaction with the cellular thiol GSH, it is likely that gliotoxin is directly reduced by cellular thiols within cells. However, a significant reduction of cellular GSH was only seen with high concentrations of gliotoxin in both hepatocytes and HSCs. It is possible, therefore, that at high cellular concentrations of gliotoxin, GSH reduces gliotoxin (oxidizing GSH to GSSG), resulting in redox cycling of gliotoxin and generation of ROS as outlined in Supplementary Fig. 2. In hepatocytes—which additionally conjugate gliotoxin with GSH—there would be a depletion of total cellular GSH and greater pressure on the reduced GSH pool to protect cellular thiols. This may therefore be the cause of the high levels of ROS observed in hepatocytes treated with a toxic concentration of gliotoxin (but not seen in HSCs).
The MPT is constituted of cyclophylin D, ANT, and possibly the voltage-activated anion channel.39, 40 Three cysteine residues in the ANT have been shown to be susceptible to a variety of thiol-reactive agents and to modulate the activity of the MPT.39, 40 It is likely that gliotoxin directly reacts with one or more cysteine residues in the ANT in a similar fashion to diamide41 or phenylarsineoxide.39, 42 This is supported by data showing that HSC apoptosis and altered HSC ANT mobility both occurred after gliotoxin treatment and both were inhibited by DTT or PDTC. DTT could function to reverse the putative gliotoxin–ANT conjugate, because it readily reduces many protein thiols. PDTC is an unusual compound because it is able to both reduce and oxidize thiol groups.43, 44 We show that PDTC does not reduce gliotoxin but is more likely to convert any reduced gliotoxin back to the oxidized form. Interestingly, PDTC contains vicinal sulphur atoms in its structure, as does gliotoxin. PDTC may therefore compete with gliotoxin for binding to ANT and prevent gliotoxin from stimulating a MPT.
With respect to apoptosis, the mechanism of action of gliotoxin may be best considered as interfering with two pathways of TNF-α receptor signaling (Supplementary Fig. 5). TNF-α is known to stimulate an apoptotic death pathway that involves an MPT-regulated release of cytochrome c from mitochondria and activation of caspase cascades (pathway 1).12, 45 However, in many cell types—including both hepatocytes and HSC—TNF-α also activates NF-κB activation (pathway 2), which inhibits apoptosis.12, 46 Accordingly, TNF-α alone stimulates hepatocyte proliferation in vivo.16 Gliotoxin is an inhibitor of NF-κB activation through its inhibition of I-κB degradation.47 Hepatocytes treated with both TNF-α and gliotoxin therefore undergo apoptosis, likely because of an inhibition of NF-κB–dependent inhibition of apoptosis. However, although gliotoxin is able to inhibit TNF-α–inducible NF-κB activity, activated HSCs contain a constitutively activated level of NF-κB activity through a CBF-1–dependent down-regulation of I-κB levels, which presumably results in a stoichiometric excess of Rel: I-κB protein.5, 7, 48 Gliotoxin treatment of HSCs therefore does not inhibit constitutive levels of NF-κB in activated HSC (note the same situation may not be the case in quiescent HSCs). The stimulation of apoptosis by gliotoxin in activated HSCs must therefore be independent of an inhibition of I-κB degradation.
In the context of liver fibrosis, these observations are important for understanding the potential mechanisms for therapeutic intervention. The HSC is pivotal to the development of liver fibrosis, and stimulation of HSC apoptosis is a potential avenue for treatment. Because cytokines such as TNF-α are known to be elevated in the diseased and fibrotic liver, an inhibition of NF-κB by any potential therapeutic approach is likely to promote the death of hepatocytes with potentially catastrophic consequences.49 However, in view of the potent effect of gliotoxin in stimulating HSC apoptosis, an analogue that retained pathway 1/MPT promoting activity without inhibiting pathway 2/26S proteasomal I-κB degradation (see Supplementary Fig. 3) could be a valuable tool in finding a treatment for liver fibrosis.
- 7Gliotoxin stimulates the apoptosis of rat and human hepatic stellate cells in vitro. In: WisseE, KnookDL, FraserR, eds. Cells of the Hepatic Sinusoid. Volume 8. Leiden, The Netherlands: Kupffer Cell Foundation, 2001: 287–290., , , , , .
- 17Persistent activation of nuclear factor-kappaB in cultured rat hepatic stellate cells involves the induction of potentially novel Rel-like factors and prolonged changes in the expression of IkappaB family proteins. HEPATOLOGY 1999; 30: 761–769., , , , , , et al.
- 432-mercaptoethanol restores the ability of nuclear factor kappa B (NF kappa B) to bind DNA in nuclear extracts from interleukin 1-treated cells incubated with pyrollidine dithiocarbamate (PDTC). Evidence for oxidation of glutathione in the mechanism of inhibition of NF kappa B by PDTC. Biochem J 1996; 320: 975–981., .
Supplementary material for this article can be found on the H EPATOLOGY website ( http://interscience.wiley.com/jpages/0270-9139/suppmat/index.html ).
|suppfig1.tif||1824K||DAPI staining of hepatocytes and activated HSCs. Cells were treated for 3 hr with gliotoxin (concentration as indicated) or 20ng/ml TNFa / 10µM cycloheximide (TNFa/CHX) for 16 hr followed by DAPI staining as outlined in methods section. Data typical of at least 3 separate experiments.|
|suppfig2a.tif||1117K||Gliotoxin metabolism in hepatocytes and HSCs. A, Hepatocytes and activated HSCs were prepared a cultured in 6 well plates as outlined in Materials and Methods section. Culture medium was removed and the cells were washed twice with 1.5 ml of HEPES/HBSS buffer. Hepatocytes were then incubated with 1.5ml of pre-warmed HEPES/HBSS buffer containing 50µM gliotoxin - hepatocytes (?) or activated HSCs (?). Cells were returned to an humidified incubator at 37oC and HEPES/HBSS medium samples were taken at various times and directly analyzed by HPLC. No change in gliotoxin concentration occured when gliotoxin was incubated in HEPES/HBSS buffer in culture plates that contained no cells (data not shown). Inset, effect of initial gliotoxin concentration on the accumulation of gliotoxin after 45 minutes incubation in hepatocytes (?) or activated HSCs (?), mean and standard deviation of 3 samples from the same experiment. Data typical of 3 separate experiments.|
|suppfig2b.tif||2202K||Gliotoxin metabolism in hepatocytes and HSCs. B, HPLC chromatograms of 50µM gliotoxin in (i) HEPES/HPLC buffer; (ii) after incubation with hepatocytes for 45 minutes; (iii) 10µM gliotoxin incubation with activated HSCs for 120 minutes and iv) 50µM gliotoxin incubation with activated HSCs for 120 minutes.|
|suppfig2c.tif||2202K||Gliotoxin metabolism in hepatocytes and HSCs. C. Timecourse for the levels of gliotoxin metabolites produced by hepatocytes incubated with 50µM gliotoxin. Concentrations of metabolites are determined assuming an identical extinction coefficient as gliotoxin at the detecting wavelength of 260nm. Data from one experiment typical of at least 4 separate experiments.|
|suppfig3a.tif||994K||Effect of gliotoxin on the levels of glutathione in a cell-free system, hepatocytes and activated HSCs. A. GSH (50µM) in HEPES/HBSS buffer was incubated with 50µM gliotoxin (+ GLIOTOXIN) or DMSO vehicle solvent (+ DMSO) at room temperature. At various times, samples were withdrawn and derivatized as outlined in the methods section and GSH and GSSG levels determined by HPLC. Data are expressed as equivalents of GSH (i.e. GSSG is equivalent to 2 times GSH); "gliotoxin conjugate?" not detected, determined after calculating recoveries.|
|suppfig3b.tif||2202K||Effect of gliotoxin on the levels of glutathione in a cell-free system, hepatocytes and activated HSCs. B. HPLC analysis of 250µM gliotoxin in HEPES/HBSS buffer incubated for 1 hour with i) no furthur addition; ii) 500µM DTT; iii) 500µM GSH µM or iv) 500µM PDTC. Chromatograms for v) DTT alone; vi) GSH alone or vii) PDTC alone. Chromatograms are for the same injection volume and are presented on identical Y axis (absorbance) scales.|
|suppfig3c.tif||2202K||Effect of gliotoxin on the levels of glutathione in a cell-free system, hepatocytes and activated HSCs. C. Timecourse for changes in glutathione levels in hepatocytes treated with 50µM gliotoxin. Hepatocytes were treated with gliotoxin and GSH levels determined after derivatization as outlined in methods section. Data are the mean and standard deviation of 3 determinations from the same experiment typical of 3 separate experiments.|
|suppfig3d.tif||2202K||Effect of gliotoxin on the levels of glutathione in a cell-free system, hepatocytes and activated HSCs. D. Timecourse for changes in glutathione levels in activated HSCs treated with control vehicle solvent (¦), 1.5µM gliotoxin (?) or 50µM gliotoxin (?). GSH levels were determined after derivatization as outlined in methods section. Note that GSSG was not detected in HSCs. Data are the mean and standard deviation of 3 determinations from the same experiment typical of 3 separate experiments.|
|suppfig3e.tif||984K||Effect of gliotoxin on the levels of glutathione in a cell-free system, hepatocytes and activated HSCs. E. Levels of glutathione in hepatocytes and activated HSCs after treatment with the indicated concentration of gliotoxin (GT) or with 20ng/ml TNFa + 10µM cycloheximide (TNFa/CHX), 100nM microcystin (MC), 200µM chlorpromazine (CLPRZ), 1mM N-ethylmaleimide (NEM) (all for 3 hours except TNFa/CHX - for 16 hours). Control hepatocytes were found to contain 20 ± 1.5 nmole GSH per mg protein and 1 ± 0.1 nmole GSSG per mg protein. Control activated HSCs were found to contain 12 ± 1. 5 nmoles GSH per mg protein. Data are the mean and standard deviation of at least 3 separate determinations. *Significantly different level of GSH or GSSG versus equivalent control treated cells, P> 95% using Student's t test (two tailed).|
|suppfig4.tif||2203K||Mechanism of toxicity of gliotoxin in rat hepatocytes. Inset, structure of gliotoxin and abbreviated structure showing the dithiol bridge.|
|suppfig5.tif||2202K||Pathways of gliotoxin mediated apoptosis. This figure is a simplification of the pathways involved in TNFa mediated apoptosis in sensitive cells.|
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