Arsenic trioxide inhibits transforming growth factor-β1-induced fibroblast to myofibroblast differentiation in vitro and bleomycin induced lung fibrosis in vivo
© Luo et al.; licensee BioMed Central Ltd. 2014
Received: 11 September 2013
Accepted: 10 February 2014
Published: 24 April 2014
Idiopathic pulmonary fibrosis (IPF) is a progressive disease of insidious onset, and is responsible for up to 30,000 deaths per year in the U.S. Excessive production of extracellular matrix by myofibroblasts has been shown to be an important pathological feature in IPF. TGF-β1 is expressed in fibrotic lung and promotes fibroblast to myofibroblast differentiation (FMD) as well as matrix deposition.
To identify the mechanism of Arsenic trioxide’s (ATO)’s anti-fibrotic effect in vitro, normal human lung fibroblasts (NHLFs) were treated with ATO for 24 hours and were then exposed to TGF-β1 (1 ng/ml) before harvesting at multiple time points. To investigate whether ATO is able to alleviate lung fibrosis in vivo, C57BL/6 mice were administered bleomycin by oropharyngeal aspiration and ATO was injected intraperitoneally daily for 14 days. Quantitative real-time PCR, western blotting, and immunofluorescent staining were used to assess the expression of fibrotic markers such as α-smooth muscle actin (α-SMA) and α-1 type I collagen.
Treatment of NHLFs with ATO at very low concentrations (10-20nM) inhibits TGF-β1-induced α-smooth muscle actin (α-SMA) and α-1 type I collagen mRNA and protein expression. ATO also diminishes the TGF-β1-mediated contractile response in NHLFs. ATO’s down-regulation of profibrotic molecules is associated with inhibition of Akt, as well as Smad2/Smad3 phosphorylation. TGF-β1-induced H2O2 and NOX-4 mRNA expression are also blocked by ATO. ATO-mediated reduction in Smad3 phosphorylation correlated with a reduction of promyelocytic leukemia (PML) nuclear bodies and PML protein expression. PML-/- mouse embryonic fibroblasts (MEFs) showed decreased fibronectin and PAI-1 expression in response to TGF-β1. Daily intraperitoneal injection of ATO (1 mg/kg) in C57BL/6 mice inhibits bleomycin induced lung α-1 type I collagen mRNA and protein expression.
In summary, these data indicate that low concentrations of ATO inhibit TGF-β1-induced fibroblast to myofibroblast differentiation and decreases bleomycin induced pulmonary fibrosis.
Idiopathic pulmonary fibrosis (IPF) is a chronic, progressive and fatal disease . A recent study indicated that the 5-year survival of IPF ranges from 30% - 50%. Despite tremendous progress in our understanding of the pathogenesis of IPF, no effective medicinal treatment has been shown to improve the mortality in afflicted patients . A prominent pathological feature of IPF is the formation of fibrotic foci, which consist of myofibroblasts and the extracellular matrix which they produce. Myofibroblasts are the principle effecter cells synthesizing pro-fibrotic proteins such as α-SMA, type I collagen, and fibronectin. Although multiple types of cells can differentiate into myofibroblasts, fibroblast to myofibroblast differentiation (FMD) is the major source for myofibroblast accumulation .
Transforming growth factor (TGF)-β1 is a potent fibrogenic cytokine and plays a crucial role in the pathogenesis of pulmonary fibrosis . TGF-β1 induces FMD by activating Smad3 and Akt signaling pathways [5, 6]. Over-expression of TGF-β1 using of a recombinant adenovirus vector carrying an active TGF-β1 construct is sufficient to induce pulmonary fibrosis in vivo . In addition, interventions that inhibit TGF-β1 signaling have been shown to block the development pulmonary fibrosis in animal models . To date there are no approved therapies to target TGF-β1 for the treatment of pulmonary fibrosis, so furthering our understanding of the profibrotic effects of TGF-β1 may lead to an effective therapy for pulmonary fibrosis.
Arsenic trioxide (ATO) has been used as a drug for more than 2000 years for the treatment of diseases including ulcers, psoriasis, and malaria . In the modern era, arsenic has been shown to be effective for the treatment of various cancers, especially acute promyelocytic leukemia (APL) [9, 10]. Recent studies have shown that ATO can regulate the expression of various proteins as well as pathways involved with TGF-β1 signaling. For example, ATO induces SnoN/SkiL, an inhibitory TGF-β1 regulator by affecting Smad3 nuclear transportation in ovarian carcinoma cells . ATO has also been reported to induce TG-interacting factor (TGIF), which is another well-characterized Smad co-repressor for TGF-β1 responsive genes. Interestingly, ATO also degrades promyelocytic leukemia (PML) nuclear bodies and PML protein expression in various cancer cell lines .
PML was originally identified as a fusion partner of retinoic acid receptor alpha (RARα) in APL patients . PML protein contains an N-terminus RING finger, two B-boxes and a coiled-coil domain, which are encoded by the first 3 exons of the PML gene. Seven different isoforms differ from each other in the C-terminus, which are generated by alternative splicing from exon 4 to exon 9. PML proteins exist in both the cytoplasm and nucleus. However, the majority of PML protein locates to the nucleus and forms complicated protein structures known as PML nuclear bodies. PML nuclear bodies are dynamic structures with diameters ranging from 200 nm to 1 μm. They exist in almost all mammalian cells and play important roles in DNA damage repair, transcription regulation, viral defense, control of apoptosis and senescence [14, 15]. PML may also regulate TGF-β1 signaling, as cytoplasmic PML (cPML) has been shown to aid with Smad3 phosphorylation in mouse embryonic fibroblasts (MEFs) by facilitating interactions among Smad anchor for receptor activation (SARA), Smad3 and the Type-I TGF-β1 receptor . However, to date the role of PML in TGF-β1-induced FMD and lung fibrosis in vivo has not been addressed.
To better understand the potential effect of ATO in regulating TGF-β1-induced FMD and lung fibrosis, we investigated how TGF-β1 signaling pathways were regulated in normal human lung fibroblasts (NHLFs) in response to treatment with ATO. We observed that ATO inhibited TGF-β1 signaling by inhibition of Smad2/Smad3 and Akt phosphorylation. We also examined the anti-fibrotic effect of ATO in vivo by using a murine bleomycin model of pulmonary fibrosis, and found that intraperitoneal administration of ATO reduced bleomycin induced pulmonary fibrosis in C57/BL6 mice.
Reagents and antibodies
Arsenic trioxide (Sigma-Aldrich) was prepared in 1 N NaOH at 250 mM and then diluted in sterile water for a stock concentration of 1 μM. Cell culture medium, FGM-2 and DMEM, were purchased from Lonza (Allendale, NJ) and Gibco. Human recombinant TGF-β1 was purchased from R&D systems (Minneapolis, MN). Antibodies used were: alpha-SMA (Sigma-Aldrich, 1:10,000), type-1 collagen (abcam, 1:2000), PML (Santa Cruz, 1:500), PAI-1 (peprotech, 1:2000), fibronectin (BD science, 1:500). Antibodies for Smad2, p-Samd2, Smad3, p-Smad3, Akt, p-Akt, Erk, p-Erk, p38, p-p38 were purchased from Cell signaling and used at a concentration of 1:1000.
Normal human lung fibroblasts (NHLFs) were purchased from Lonza (Allendale, NJ). Cells were maintained in FGM-2 (Lonza) and only early passage cells (before passage 6) were used for all experiments. Wild-typed and PML -/- mouse embryonic fibroblasts (MEFs) were a kind gift from the laboratory of Dr. Pier Paolo Pandolfi (Beth Israel Deaconess Cancer Center) and maintained in DMEM with 20% FBS and 1% penicillin-streptomycin (Gibco). Human lung fibroblasts from control patients and IPF patients were a generous gift from the laboratory of Dr. Eric S. White (University of Michigan, Ann Arbor).
Western blot analysis
Cells were harvested using 1x RIPA buffer (Cell signaling) with 1 mM PMSF (Sigma Aldrich). Thirty μg of protein per sample was loaded onto 4–12% Novex Tris-Glycine SDS polyacrylamide gels (Invitrogen) for electrophoresis and then transferred on polyvinylidene difluoride (PVDF) membranes (0.45 μm, Invitrogen). Membranes were then blocked in 5% Milk (BioRad) for 1 hour at room temperature and then incubated with the appropriate primary antibody overnight. Secondary antibodies and an ECL kit from (GE) were applied for generating chemiluminescent signals. All western blot data represents triplicate repeats. Densitometry analysis was performed using National Institutes of Health (NIH) ImageJ software.
Real time quantitative PCR
Real time quantitative PCR was performed using the iCycler (Bio-Rad Laboratories, Hercules, CA), and SYBR green supermix (Bio-Rad) was employed according to the manufacturer’s instructions. mRNA expression was corrected to expression of the 36B4 housekeeping gene. Primer sequences that were employed were: h-α-SMA: Fwd: GAAGAAGAGGACAGCACT, Rev: TCCCATTCCCACCATCAC; m-α-SMA: Fwd: TGCTGACAGAGGCACCACTGAA, Rev: CAGTTGTACGTCCAGAGGCATA; h-Collagen-1: Fwd: CGGAGGAGAGTCAGGAAGG, Rev: CACAAGGAACAGAACAGAACA; m-Collagen-1: Fwd: GCCAAGAAGACATCCCTGAAG, Rev: TCATTGCATTGCACGTCATC; 36B4: Fwd: CGACCTGGAAGTCCAACTAC; Rev: ATCTGCTGCATCTGCTTG; h-CTGF: Fwd: GGCTTACCGACTGGAAGAC, Rev: AGGAGGCGTTGTCATTGG; h-PAI-1: Fwd: GGCTGGTGCTGGTGAATGC; Rev: AGTGCTGCCGTCTGATTTGTG.
Rat tail type I collagen gel contraction assay
Rat tail type I collagen gel contraction assay was conducted as previously described . Briefly, a 12-well cell culture plate was pre-coated with 5% sterile BSA for 4 hours. Rat tail type-I collagen (354236 BD biosciences) was diluted with fibroblast basal medium (FBM, Lonza, CC-3131) with 0.5% BSA into 2 mg/ml and mixed with NHLFs to reach a final concentration of 2 × 105 cells/ml. One N NaOH was added as per the manufacture’s instruction. Eight hundred microliters of cell-collagen mixture were then added into each well of the culture plate and incubated at 37° for 30 minutes. Cells were incubated in FBM medium with 0.5% BSA overnight. Cells were treated with arsenic trioxide and TGF-β1 as indicated. Gel sizes were measured using the National Institutes of Health (NIH) ImageJ software. To harvest the cells from the gel, a type I collagenase (Invitrogen) was applied to dissolve the collagen gel. Briefly, trypsin was added onto the gels for 5 minutes. Type I collagenase (5 mg/ml) was then added onto the gels and they were incubated at 37° for 30 minutes. Cells were spun down and lysed using RIPA buffer for western blot analysis.
NHLFs were plated into 8 well chamber slides and treated as indicated. After washing in PBS for 5 minutes, cells were fixed by 4% paraformaldehyde (Electron Microscopy Sciences) for 10 minutes. Fixed cells were then washed in HBSS for 5 minutes 3 times before a blocking buffer (5% Goat serum + 0.5% BSA + 0.4% Triton X-100) was added for 1 hr at room temperature. Appropriate primary antibodies and secondary antibodies were then added for one hr at room temperature. A 10 minute HBSS wash times 3 was performed prior to the addition of the secondary antibody. DAPI (Invitrogen) was added for nuclear staining and prolong gold (Invitrogen) was used for preserving the signal.
For processing paraffin embedded tissue slides, slides were incubated at 60°C for 45 min. Then slides were de-paraffinized by immersion in xylene and re-hydrated. Following hydration, slides were boiled in 1x SSC for 10mins for antigen retrieval. After boiling slides were kept in hot SSC for 30 mins. at room temperature. Slides were then washed in 50 μM ammonium chloride for 10 mins., then rinsed in PBS for 10 mins. 3 times prior to application of the primary antibody.
An in vitro toxicology assay kit (Sigma Aldrich) was used for this experiment. Briefly, NHLFs were plated into a 12-well plate and pretreated with ATO (10nM, 20nM) for 48 hrs. Cells were then washed with HBSS prior to addition of 1 ml of FGM. MTT (M-5655, Sigma Aldrich) was added into to media and cells were incubated at 37°C for 2 hrs. Thereafter, the culture media was removed and MTT Solubilization Solution (M-8910, Sigma Aldrich) was added. Absorbance of each well was measured at the wavelengths of 570 nm and 690 nm.
NHLFs were treated with ATO and TGF-β1 as indicated. Then cells were incubated with 30 μM DCFH-DA at 37°C for 30 min. and washed with HBSS several times. Cells were lysed in 1 N NaOH and the intensity of fluorescence was determined using a plate reader with an excitation filter at 485 nm and an emission filter at 535 nm. The H2O2 level was calculated as the mean fluorescence intensity of each sample.
Cytoplasmic and nuclear protein extraction
Proteins from cytoplasm and nucleus compartments were separated by using NE-PER Nuclear and Cytoplasmic Extraction Reagents (Thermo scientific, #78835). Briefly, NHLFs were harvested with trypsin-EDTA and then washed twice with PBS. Then cells were centrifuged at 500 × g for 5 minutes and supernatants were removed. Ice cold CER-I and CER-II solutions were added per the manufacturer’s instructions to separate the cytoplasmic from the nuclear compartment proteins. Western blot for GAPDH and histone 3 were used to ensure there was no contamination in each part of the extracts.
Bleomycin and ATO treatment
All protocols for animal studies were approved by the Institutional Animal Care and Use Committee of Tulane University. C57/BL6 mice (Charles River) were separated into 5 groups with 7 mice in each group. Two days before bleomycin exposure, arsenic trioxide (1 mg/kg) was administered daily by intraperitoneal injection in the ATO-pretreatment group. PBS with the same amount of NaOH employed to solubilize the ATO was used as a control for other groups. Bleomycin (Zhejiang Hisun Pharmaceutical Co., Ltd, 2units/kg) was given by oropharyngeal aspiration as described previously (25). For the ATO-delayed treatment group, ATO was administered daily starting on day 6 following bleomycin administration. Mice were sacrificed on day 14 after administration of bleomycin. Left lungs were fixed for trichrome staining and right lungs were harvested and homogenized in liquid nitrogen for real time quantitative PCR and western blot analysis.
Total collagen quantification
Left lungs were paraffin-embedded and tissue slides were prepared for trichrome staining. An Aperio slide scanner (Aperio, CA) was used to scan the tissue slides per the manufacturer’s instruction. The whole lung tissue section on a single slide was scanned and collagen content was calculated using an internal PPC Collagen (2) RWB program. A ratio of total positive value to the total number value was used to represent collagen expression.
Statistic analysis was conducted using ANOVA followed by the Bonferroni post hoc test. Data are presented as the mean (±SEM) and represent multiple experiments performed in triplicate.
ATO inhibits TGF-β1 induced fibrotic markers
NHLFs have a spindle-shaped morphology while myofibroblasts are more stellar shaped cells and express α-SMA in fibrils . NHLFs were pretreated with ATO (10nM, 20nM) for 24 hrs and then treated with TGF-β1 (1 ng/ml) for another 24 hrs, to test whether ATO affects TGF-β1-induced. α-SMA fiber formation. Immunofluorescent staining demonstrated that ATO pretreatment decreased TGF-β1 induced incorporation of α-SMA into fibrils (Figure 1F). ATO is a well-characterized inducer of apoptosis in APL as well as non-malignant cell lines [20, 21]. Recent studies have shown that ATO induces pulmonary fibroblast growth inhibition at a concentration of 50 μM . However the concentration of ATO used in our studies are several orders of magnitude lower than the concentration employed in the manuscripts mentioned above. To examine whether 10nM or 20nM concentrations of ATO inhibit NHLF cell viability, cells were treated with ATO for 48 hrs and protein was harvested for western blot. An MTT assay revealed no significant differences in cell viability when cells were exposed to these low concentrations of ATO (Figure 1G).
ATO inhibits TGF-β-induced fibroblast contractile activity
ATO inhibits Smad2/Smad3 and Akt phosphorylation
To assess whether ATO down-regulates TGF-β1-driven phosphorylation on a global level, we also evaluated P38 phosphorylation, which is also involved in TGF-β1 signaling . NHLFs were pretreated with ATO (10nM or 20nM) for 24 hrs and treated with TGF-β1 for 30 mins. p38 phosphorylation was induced by TGF-β1 and ATO pretreatment did not diminish its phosphorylation (Figure 3E). This indicates that ATO does not globally affect phosphorylation. Erk phosphorylation was also assessed, however, we did not observe an increase in Erk phosphorylation in the NHLFs in response to TGF-β1 over several time points, nor a diminution in the baseline Erk phosphorylation in response to ATO.
ATO blocks TGF-β1 induced H2O2and NOX-4 mRNA expression
Reactive oxygen species (ROS), especially H2O2 plays an important role in the derivation of TGF-β1-mediated fibrotic phenotypes . To investigate whether low doses of ATO regulate H2O2 levels in NHLFs, we pretreated the cells with ATO (10nM or 20nM) for 24 hrs and then exposed them to TGF-β1 for another 12 hrs. These low concentrations of ATO did not induce H2O2 (0.81 ± 0.04 & 0.77 ± 0.04; p > 0.05), and to the contrary, TGF-β1-induced H2O2 expression was blocked by ATO (1.11 ± 0.04 & 0.95 ± 0.07 vs. 1.49 ± 0.06; p < 0.05) (Figure 3F). To investigate whether ATO down-regulated TGF-β1 induced Smad3 phosphorylation by reducing H2O2 expression, NHLFs were pretreated with ATO (20nM) for 24 hrs and then exposed to TGF-β1 with or without H2O2 (100 μM, 200 μM, and 300 μM) for an addional 30 mins. H2O2 (100 μM) partially restored Smad3 phosphorylation reduced by ATO (Figure 3G). The NADPH oxidase (NOX) proteins generate H2O2 by transferring electrons to oxygen, and NOX-4 has been reported to mediate myofibroblast differentiation [25, 26]. To determine how ATO regulates TGF-β1 induced NOX-4 expression, NHLFs were pretreated with ATO (10nM or 20nM) for 24 hrs and then treated with TGF-β1 (1 ng/ml) for another 24 hrs. TGF-β1 induced a marked up-regulation of NOX-4 mRNA (264.80 ± 19.29; p < 0.05), however pre-treatment with ATO significantly blunted this effect (119.50 ± 17.66 & 136.20 ± 28.32 vs. 264.80 ± 19.29; p < 0.05) (Figure 3H).
ATO causes a reduction in PML protein and PML nuclear bodies in NHLFs
PML is essential for TGF-β signaling in MEFs
To test whether PML is essential for TGF-β1 signaling and Smad phosphorylation, wild type MEFs and PML -/- MEFs were treated with TGF-β1 (1 ng/ml) for 24 hrs and harvested for western blot analysis. TGF-β1 induced PAI-1 and fibronectin protein expression in wild-type MEFs; however the induction decreased in PML -/- MEFs (Figure 4C). TGF-β1 induces the phosphorylation of both Smad2 and Smad3 but the profibrotic effect induced by TGF-β1 is largely dependent on Smad3 activation . To investigate whether PML plays a role in Smad3 activation, wild type MEFs and PML -/- MEFs were treated with TGF-β1 (1 ng/ml) for the indicated time points. Smad3 phosphorylation was induced by TGF-β1 in the wild type MEFs and this event was markedly decreased in PML -/- MEFs (Figure 4D).
ATO inhibits bleomycin induced lung fibrosis in C57BL/6 mice
In this study, we have demonstrated that ATO inhibits TGF-β1 induced FMD, as well as type-I collagen and α-SMA expression. We also have shown that ATO reduces bleomycin-mediated pulmonary fibrosis in mice. As for the mechanism, we found that ATO down-regulates Smad2/Smad3 and Akt phosphorylation in vitro. We also showed that ATO decreased PML expression in NHLFs, which could in turn regulate Smad3 phosphorylation. ATO has very recently been shown to be protective against bleomycin- induced fibrosis by subcutaneous injection in BALB/c mice , which further supports our hypothesis that ATO could be used as an anti-fibrotic agent. Our study provides more detailed and profound description of ATO’s anti-fibrotic effect by illustrating the mechanisms in vitro, and employs a 5-times lower dose (1 mg/kg) of ATO, as well as, a more bleomycin more susceptible mouse strain for the in vivo studies . What is more, our experimental design included early and late administration of ATO following lung injury, and makes an association with PML body expression.
The dose of ATO is critical for its potential therapeutic application for the treatment of pulmonary fibrosis. At concentrations in the micromolar range, ATO induces ROS and promotes apoptosis for fibroblasts and other primary cells [22, 31–33]. ATO can also induce acute airway epithelial injury by altering ATP-dependent Ca2+ signaling . Furthermore, intravenous injection of ATO (1 mg/kg) was reported to induce cardiac fibrosis . However, ATO concentration in the nanomolar range, as we used in this study, is less toxic. The MTT assay indicates that ATO at 10nM and 20nM does not change the NHLF viability. The report of cardiac fibrosis had not been published at the time we conducted our in vivo experiments, and although we did not note a cardiac effect on chest dissection we were not specifically looking for one. ROS, especially H2O2, are considered to be profibrogenic and are induced by TGF-β1 through a mechanism that involves up-regulation of NOX-4 activity . However, ATO at 10nM and 20nM did not induce H2O2, but conversely blocked TGF-β1 induced NOX-4 mRNA and H2O2 expression. In addition, in the ATO treatment alone group, there were no observed untoward histological changes. Of relevance, the concentration we used in our study is several orders of magnitude lower than the clinical application of ATO for the treatment of APL .
Fibroblast to myofibroblast differentiation (FMD) is a crucial step for the genesis of myofibroblasts. Myofibroblasts are the effecter cells for producing extra-cellular matrix in fibroblastic foci which lead to loss of alveolar function of IPF lungs . Myofibroblasts secrets α-SMA, a stress fiber not only affects the compliance of lungs but also works as a signal transduction molecule to regulate extracellular matrix proteins production . Myofibroblasts also contribute to abnormal epithelial functions and induce epithelial apoptosis by secreting pro-inflammatory cytokines . Instead of directly inducing apoptosis of fibroblasts, we have shown that low dose of ATO blocked expression of multiple TGF-β1-induced myofibroblast markers as well as mRNA levels of potent profibrotic cytokines and proteins such as CTGF and PAI-1.
Smad and Akt activation are two key pathways involved in the development of TGF-β1-induced fibrogenic phenotypes. A previous study has shown that ATO at concentrations of 10 μM diminishes Smad3 protein expression . Although knocking down basal Smad3 expression might be beneficial for blocking TGF-β1 induced FMD, loss of Smad3 has been reported to correlate with enlargement of airspaces and development of emphysema . In this study, we show that ATO in the nanomolar range inhibits TGF-β1 induced Smad3 phosphorylation, but does not decrease Smad3 expression. ATO has also been reported to inhibit Akt phosphorylation at a concentration of 3 μM in lymphoma B cells . Consistent with that study, we observed that a low concentration of ATO inhibits TGF-β1 induced Akt phosphorylation in NHLFs. The experiment in which ATO was washed away prior to adding TGF-β1 excludes the possibility of TGF-β1 ligand inactivation as an explanation for the inhibition of Smad and Akt phorphorylation. Moreover, ATO does not inhibit phosphorylation in a global level, as the experimental data show that Erk and p38 phosphorylation are not diminished in response to ATO.
To investigate how Smad3 phosphorylation is affected by ATO, we focused on PML, a protein reported to be degraded by ATO . Consistent with a previous study , we found that TGF-β1-induced PAI-1 and fibronectin expression as well as Smad3 phosphorylation were all impaired in PML -/- MEFs. To further test our hypothesis that PML knockdown by ATO may be responsible for an impaired TGF-β1 signaling in NHLFs, a “rescue” experiment to transfect PML plasmid into NHLFs in an attempt to restore TGF-β1 signaling was considered. However, ATO can efficiently induce the oligomerization of PML, which promotes its ubiquitination and degradation . Thus, we did not pursue this approach because exogenous PML would be expected to be degraded by ATO in a similar manner. In addition to the important role of cPML in TGF-β1 signaling, PML may have profound impact on the pathogenesis of IPF via induction of cellular senescence through interactions with p53 and Rb . Accelerated epithelial senescence has been observed in IPF lungs compared to control lungs . Furthermore, PML functions as a negative regulator of hTERT and therefore contributes to short telomere length , and short telomeres have been reported to be a risk factor for IPF [33, 42]. Taken together, PML may play a key role in the pathogenesis of IPF, but further experiments will need to be conducted to test this concept. In addition to PML, we have also shown that H2O2 might also play a role in ATO’s reduction on TGF-β1 induced Smad3 phosphorylation. H2O2 (100 μM) partially restored ATO reduced Smad3 phosphorylation. How ATO regulates H2O2 and Nox4 expression is an area of interest to us for future studies.
Lastly we have shown that ATO inhibits bleomycin-induced fibrosis in vivo. We have shown that 1 mg/kg of ATO is able to significantly reduce the expression of PML bodies in C57BL/6 mouse lungs, as it blocks bleomycin induced type-1 collagen, and diminishes the basal level of α-SMA expression in mouse lungs. The delayed treatment group has a slightly better effect compared with the pre-treatment group. One possible explanation for this may be associated with the massive DNA damage induced by bleomycin to the epithelial cells  and PML bodies are actively involved in the DNA repair process. Thus, the absence of PML bodies at the time of DNA injury could lead to sustained epithelial cell dysfunction and possibly a higher level of pro-inflammatory cytokines . Future experiments, are planned that will employ PML KO mice in murine models of pulmonary fibrosis.
In summary, this work demonstrates that ATO effectively inhibits TGF-β1 induced FMD in vitro and reduces lung fibrogenesis in vivo. Although the ATO concentrations employed in these experiments were low and ATO is already an FDA approved drug, it is unclear whether or not trials using low dose ATO for the treatment of recalcitrant and deadly diseases such as IPF would be considered an acceptable form of therapy.
We would like to thank Dr. Pier Paolo Pandolfi for generously providing the PML null and wild type MEF cell lines. We would also like to thank Dr. Yongli Shi and Hong Nguyen for helping with the experiments. This work is supported, in part or in whole, by Wetmore Foundation. Dr. Cecilia G. Sanchez was partially founded by COBRE NIH/NIGMS P20GM103629.
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