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From the Receptor Biology Laboratory,* Toxicology and Molecular Biology Branch, and the Experimental Pathology Laboratory, Pathology and Physiology Research Branch, Health Effects Laboratory Division, National Institute for Occupational Safety and Health, Centers for Disease Control and Prevention, Morgantown, West Virginia
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Abstract |
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Whereas NF-E2 is strictly expressed in hematopoitic cells and is required for regulation of ß-globin gene expression, Nrf2 is ubiquitously expressed in animal tissues, and its role in ß-globin expression remains uncertain.9 Instead, increasing evidence reveals that Nrf2 mediates the antioxidant response element (ARE)-dependent transcriptional regulation of a battery of genes. These include phase II enzymes such as NAD(P)H:quinine oxidoreductase 1 (NQO1) and glutathione S-transferase A1 (GSTA1), which detoxify endogenous and exogenous chemicals through reduction and conjugation reactions, and antioxidative enzymes and proteins such as thioredoxin, heme oxygenase 1 (HO-1), and ferritin, which participate in reactive oxygen species (ROS) metabolism or directly scavenge ROS. Thus, Nrf2 appears to function as a key regulator of the antioxidant response. Consistent with this notion, a number of genetic studies have implicated Nrf2 in a range of protective responses against chemical-induced lesions or disease states. Loss of function of Nrf2 is associated with increased sensitivity to chemical carcinogenesis such as benzo(a)pyrene-induced gastric neoplasia,10 acetaminophen-induced hepatotoxicity,11 hyperoxic lung damage,12 pulmonary injury by butylated hydroxytoluene13 or diesel exhaust,14 and premature ovarian failure by the occupational ovotoxicant 4-vinyl cyclohexine diepoxide.15 Although Nrf2 is dispensable for life in mice, it cooperates with Nrf1 to regulate antioxidant gene expression during early embryonic development. A combined deletion of Nrf1 and Nrf2 results in marked oxidative stress and increased apoptosis in the liver leading to embryonic lethality, suggesting overlapping functions among the CNC bZip proteins and possibly compensation for each other in the defense against oxidative stress during embryonic hepatogenesis.16
The molecular mechanism of Nrf2 action is best understood for the induction of phase II genes, such as the induction of Nqo1 by phenolic antoxidants.17,18 In the absence of an activator, Nrf2 is a labile protein localized in the cytoplasm forming a complex with Keap1. Keap1 anchors Nrf2 in the cytoplasm by interacting with cytoskeletal proteins. Moreover, Keap1 regulates the ubiquitin-26S proteasome-mediated turnover of Nrf2 through a Cul3-based E3 ligase. Binding of tert-butylhydroquinone (tBHQ) to Keap1 stabilizes Nrf2. Activated Nrf2 translocates into the nucleus and forms a heterodimer with a Maf protein. The dimer then binds to AREs located in the enhancer regions and mediates the transcription of the genes. Variations of this Nrf2/ARE paradigm have been observed in the transcriptional regulation of a number of genes, suggesting high adaptability of Nrf2 action in a broad range of biological functions. For instance, Nrf2 can interact with activating transcription factor 4 in the induction of Ho-1,19 compete with Jun/Fos for binding to ARE/AP1 sites in the induction of thioredoxin by hemin,20 or cross-interact with aryl hydrocarbon receptor (AhR) signaling for induction of murine Nqo1 by AhR agonist 2,3,7,8,-tetrachlorodibenzo-p-dioxin (TCDD).18
Here, we report that loss of Nrf2 in mice is associated with the development of autoimmune-mediated lesions in multiple tissues. The lesions were characterized by disseminated inflammation, appearance of anti-double-stranded DNA (dsDNA) antibodies at young ages, vascular deposition of immunoglobulin complexes, and premature death due primarily to rapidly progressing glomerulonephritis. Surviving mice frequently died of neoplasia of lymphoid, histiocytic, or endothelial origins. Nrf2-null mice exhibited increased proliferative response of CD4+ cells and altered ratios of CD4+ and CD8+ peripheral T cells. Finally, the Nrf2-null mice were devoid of the basal and inducible expression of a number of phase II and antioxidant-responsive genes and concomitantly displayed increased oxidative lesions in multiple tissues. Together, the findings suggest interplay between Nrf2 function, ROS defense, and autoimmune surveillance in the development of autoimmune disorders.
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Materials and Methods |
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Nrf2 knockout mice (kindly provided by Dr. Y.W. Kan, University of California, San Francisco, CA) were re-derived at Jackson Laboratory to assure specific pathogen-free status.18 Nrf2–/– and Nrf2+/+ mice on a genetic background of 129SVJ were maintained at an environmentally controlled National Institute for Occupational Safety and Health animal facility, which is fully accredited by the Association for Assessment and Accreditation of Laboratory Animal Care International. The mice were barrier maintained with a light/dark cycle of 12 hours at a constant temperature (22°C) in HEPA-filtered, individually ventilated microisolator cages (Thoren Caging Systems, Hazleton, PA). Irradiated food (6% fat; 7913; Harlan-Teklad, Madison, WI) and water were provided ad libitum. Bedding was sterile Beta chip from Northeastern Products Company (Warrensburg, NY). Mice were observed daily for signs of illness. Moribund mice showing severe edema or lethargy were sacrificed for histopathological examinations. Mouse breeding, morbidity, and mortality were recorded using the Colony software, version 3.0 (Locus Technology, Inc., Orland, ME).
Isolation of Peripheral Lymphocytes and Flow Cytometry Analysis
Lymph nodes (from the mandibular and axillary regions) and spleen were collected. Lymphocytes were isolated by gentle disruption of the tissues with the flat end of a syringe plunger against the bottom of a 70-µm nylon cell strainer (Becton Dickinson Labware, Franklin Lakes, NJ), followed by centrifugation at 1200 x g for 10 minutes. Red blood cells in spleen samples were removed by lysis with ammonium chloride lysing reagent (BD Pharmingen, San Diego, CA) and repeated centrifugation and washing. CD4+, CD8+, or CD45R/B220+ cells were isolated using BD IMagnet according to manufacturer’s instructions (BD Pharmingen). Briefly, an appropriate number of lymph node cells or splenocytes were suspended in 1x BD IMag buffer and blocked for nonspecific binding with anti-mouse CD16/CD32 monoclonal antibody (BD Pharmingen) on ice for 15 minutes, followed by a brief spin. Cell pellets were re-suspended in 0.5 ml of IMag buffer, mixed with 50 µl of BD IMag anti-mouse CD4, CD8a, or CD45R/B220 particles, and incubated at 4°C for 30 minutes. The cells labeled with IMag particles were placed in the BD IMagnet and were separated from unlabeled cells by magnetic force. The separation process was repeated one more time. Isolated CD4+, CD8+, or CD45R/B220+ cells were examined for purity by fluorescence-acitvated cell sorter (FACS) as described below and were used for cell proliferation and FACS analysis.
For staining of cell surface antigens, 
5 x 105 to 1 x 106 cells were blocked with anti-mouse CD16/CD32 on ice for 15 minutes. The cells were then stained with R-phycoerythrin-conjugated anti-mouse CD4, flourescein isothiocyanate (FITC)-conjugated anti-mouse CD8a, or peridinin chlorophyll-
protein-conjugated anti-mouse CD45R/B220 monoclonal antibodies (BD Pharmingen) on ice in the dark for 15 minutes. After washing, the cells were resuspended in staining buffer and analyzed using FACSCalibur (Becton Dickinson, San Jose, CA).
Lymphocyte Proliferation Assay
To analyze responses of lymphocytes to proliferative stimuli, splenocytes, lymph node cells, or isolated CD4+, CD8+, and CD45R/B220+ cells were cultured in RPMI 1640 (Invitrogen, Carlsbad, CA) supplemented with 4 mmol/L glutamine and 10% fetal bovine serum. To measure response to anti-CD3, cells (5 x 104 or 1 x 105) were seeded in a 96-well BD BioCoat T-Cell Activation Plate precoated with anti-CD3 antibodies (BD Discovery Labware, San Diego, CA) and incubated at 37°C with 5% CO2 for 48 hours. Proliferation of the cells was measured using the 3-(4,5-dimethyl thiazole-2-yl)-2,5-diphenyl tetrazolium bromid (MTT) kit from Roche Applied Science (Indianapolis, IN). MTT labeling reagent (10 µl) was added to each well, and the plate was incubated for 4 hours in a CO2 incubator, followed by adding 100 µl of a solubilization solution into each well. The plate was kept overnight in the incubator, and cell proliferation was measured at 550 nm using a plate reader (Spectra Max 340PC; Molecular Devices, Sunnyvale, CA). For B-cell proliferation assay, purified B cells were activated with goat F(ab')2 anti-mouse IgM (Jackson ImmunoResearch, West Grove, PA) or lipopolysaccharide (20 µg/ml; Sigma, St. Louis, MO) for 48 hours. Proliferation was measured with the MTT kit as described above.
Antibody Titration
Blood samples were collected from tail veins of age-matched (5- to 7-month-old) male and female Nrf2+/+, Nrf2+/–, or Nrf2–/– mice (all in the 129SVJ background) and C57BL/6J mice (as a separate control; The Jackson Laboratories, Bar Harbor, ME) into serum tubes (Becton Dickinson). Sera were prepared and measured for mouse anti-dsDNA or anti-single-stranded DNA antibodies using enzyme-linked immunosorbent assay (ELISA) kits from Alpha Diagnostic International (San Antonio, TX) according to supplier’s instructions. ELISA was measured at 450 nm using Spectra Max 340PC plate reader.
Determination of Blood Urea Nitrogen (BUN), Total Protein, and Hematocrit
Serum BUN and total protein were determined using a COBAS MIRA Plus Chemistry Analyzer (Roche Diagnostics Corp., Indianapolis, IN). Blood was collected from the abdominal vena cava, placed in a serum microtainer tube, and incubated for approximately 20 minutes. Blood was centrifuged for 15 minutes at 3000 rpm, and serum was collected and placed in a vial. The vial was then placed in the Chemistry Analyzer. BUN and total protein were determined using Reagent for BUN from Roche Diagnostics or Reagent for Total Protein from Sigma, respectively. For hematocrit determination, blood was drawn from the abdominal vena cava into standard heparinized hematocrit tubes. One end of each tube was sealed with clay tube sealer. The tubes were centrifuged on a Damon IEC MB centrifuge (Damon, Needham Heights, MA) at 13,700 x g for 5 minutes. Hematocrit was determined with a Damon microcapillary reader (Damon).
Measurement of Lipid Peroxidation
Free malondialdehyde (MDA) was measured using the Bioxytech MDA-586 kit from OxisResearch (Portland, OR). Briefly, kidney, liver, and heart tissues were collected from female Nrf2–/– or Nrf2+/+ mice at 6 months of ages or as indicated in figures. The tissues were homogenized in the presence of 5 mmol/L butylated hydroxytoluene. Extracts were prepared by centrifugation at 10,000 x g for 10 minutes. MDA contents were assayed and measured spectrophotometrically according to instructions provided by the manufacturer.
Treatment of Mice and Analysis of mRNA Expression
Nrf2+/+ and Nrf2–/– mice (2 months old) were treated with corn oil or 3-t-butyl-4-hydroxy anisol (BHA). BHA is administered by gavage on days 1 and 3 at a dose of 400 mg/kg body weight. Liver and spleen samples were collected on day 4 after BHA treatment and were stored in RNALater (Qiagen, Valencia, CA). Total RNA was prepared using a Qiagen Total RNA isolation kit (Qiagen). Northern blotting was performed as follows. RNA samples (5 µg) were fractionated in a 1% agarose-formaldehyde gel and transferred to a Nytran membrane. The blot was probed with a dioxigenin (DIG)-labeled riboprobe prepared with the DIG-labeling kit (Roche Applied Science) for mouse genes according to established procedures.21 Signals were visualized by chemiluminescence using a DIG RNA detection kit with CDP Star as a substrate (Roche Applied Science). Parallel blots of the same samples were probed with a DIG-labeled mouse actin probe to ensure equal loading. Results shown were repeated two times in separate experiments with consistent observations.
Real-time polymerase chain reaction (PCR) was performed using SYBR Green PCR master mix (Applied Biosystems, Foster City, CA) on a Bio-Rad iCycler (Bio-Rad, Hercules, CA) following standard procedures. Briefly, single-stranded cDNA was synthesized from 1 µg of total RNA using Superscript III reverse transcriptase (Invitrogen). For PCR reach reaction, 2 µl of DNA template, 2 µl of forward and reverse primers (10 µmol/L each), 25 µl of SYBR Green PCR Master Mix, and 19 µl of water were added to a final volume of 50 µl. Thermal cycling was performed as follows: 95°C for 3 minutes as initial denaturing, followed by 45 cycles of 94°C for 30 seconds, 60°C for 30 seconds, and 72°C for 60 seconds, and a final extension at 72°C for 2 minutes. Threshold cycles (CT values) were determined using the iCycler IQ software (Bio-Rad). Real-time PCR results were normalized using 1% of input as an internal control. Relative DNA amounts were calculated from the CT values for each sample by interpolating into the standard curve obtained using a series dilution of standard DNA samples run under the same conditions. Primer sets used for real-time PCR were as follows: NQO1 forward, 5'-AAC-GGGAAGATGTGGAGATG-3', and reverse, 5'-CGCAGTAGATGCCAGTCAAA-3'; HO-1 forward, 5'-GAGCAGA-ACCAGCCTGAACTA-3', and reverse, 5'-GGTACAAG-GAAGCCATCACCA-3'; and ß-actin forward, 5'-GACC-TCTATGCCAACACAGT-3', and reverse, 5'-ACTCATC-GTACTCCTGGTG-3'.
Histological, Immunofluorescent, and Electron Microscopy
Tissue samples were fixed in 10% neutral buffered formalin for 1 day, subsequently routinely processed, and embedded in paraffin. Sections of 5 µm thickness were stained with hematoxylin and eosin (H&E) or with PAS. Slides were interpreted by a board-certified veterinary pathologist blinded to the genotypes of individual animals. For immunofluorescent studies of immunoglobulin complex deposition, fresh kidneys or other tissues were flash frozen in liquid nitrogen and subsequently stored at –80°C. Frozen sections were prepared using a cryostat. Sections were washed with phosphate-buffered saline (PBS; Sigma) three times (10 minutes each), followed by a 5-minute wash with PBS. Nonspecific binding was blocked by sequential 10-minute baths in 5% PBS/bovine serum albumin (IgG free) and 5% pig serum (Biogenex, San Ramon, CA). Primary antibodies were incubated with tissue sections for 2 hours in the dark as follows: FITC-goat anti-mouse IgG+A+M (Zymed, South San Francisco, CA) 1:20 in PBS plus 10% goat serum; Alexa Fluor 488-goat anti-mouse IgG (Molecular Probes, Eugene, OR) 1:20 in PBS; Alexa Fluor 488-goat anti-mouse IgM (Molecular Probes) 1:20 in PBS; or fluorescein-conjugated goat IgG fraction against mouse complement C3 (ICN/Cappell, Aurora, OH) 1:400 in PBS. Sections were rinsed three times with PBS (each for 5 minutes), covered with coverslips in Gelmount (Biomeda, Foster City, CA), and examined under a fluorescent microscope. For transmission electron microscopy, fresh kidney samples were preserved in Karnovsky’s fixative, postfixed in osmium tetroxide, mordanted in tannic acid, and stained en bloc in uranyl acetate. The tissues were then dehydrated in alcohol and embedded in Epon. The sections were stained with uranyl acetate and lead citrate. Kidney samples were examined ultrastructurally using a JEOL 1220 electron microscope.
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Results |
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The Nrf2-null mice bred normally, and their offspring grew and matured similarly to Nrf2+/+ mice. However, the mice developed a range of signs of illness after 2 months of age (Figures 1 and 2
). Manifestations of illness were diverse, including reduced body weight, subcutaneous edema, which often started at the facial area and spread to the whole body gradually (Figure 2A)
, pale ears and toes, cutaneous ulcers, ring-shaped tail redness and necrosis (Figure 2B)
, eye inflammation (Figure 2A)
, and neurological symptoms (dysmetria, tremors, lethargy, and seizures) (Figure 2A)
. These signs were rarely observed in Nrf2+/+ mice with the same genetic background during the period of study (Figure 1A)
. Moreover, a clear female predominance of the illness was seen (Figure 1A)
. The morbidities of the female mice were 29, 79, and 100% at ages of 15, 25, and 55 weeks, respectively, whereas, those of the male were 4, 33.3, and 58.3% at the same ages (Figure 1A)
. In addition, female mice appeared to develop signs of illness earlier (10 versus 14 weeks) and more severely than their male littermates.
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. Similar to the morbidity, a clear gender-dependent difference in survival was observed. Female mice died earlier and at a higher rate than male mice. The survival rates of the female at ages of 15, 25, and 55 weeks were 71.4, 50, and 21.4%, respectively, substantially lower that those of the male (ie, 96, 87.5, and 58.3% at the same ages). Thus, loss of Nrf2 in mice caused a spontaneous, gender-dependent, and diverse spectrum of disease manifestations and mortality in the absence of apparent exposure to exogenous toxic chemicals. Glomerulonephritis
Histopathological examination of the diseased mice revealed a high prevalence of glomerulonephritis. Among the mice that died or were euthanized because of severe illness, the glomerulonephritis prevalence was 88% (31 with glomerulonephritis, 3 without glomerulonephritis, and 1 unevaluated because of extensive tissue autolysis). The mean age of Nrf2-null mice with glomerulonephritis was 9 ± 1 (SE) months with a range of 2 to 22 months. Glomerulonephritis was the primary cause of death in 69% (22 of 32) of Nrf2-null mice in this necropsy series, causing death in mice as young as 2 months of age. Glomerulonephritis was seen in both female and male mice and was the cause of death in 88% (15 of 17) of female and 47% (7 of 15) of male mice. Spontaneous death was often accompanied by subcutaneous edema and lethargy. The corresponding histopathological alterations seen in affected Nrf2-null mice were varying manifestations of membranoproliferative glomerulonephritis (Figure 3)
. Antemortem BUN concentration was elevated in mice with the most severe histopathological changes in glomeruli (Figure 4)
. In wild-type and heterozygous mice, membranoproliferative glomerulohephritis was uncommon, and signs of renal failure were not observed.
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. The severity of the kidney lesions often correlated with age and morbidity. In older mice and those with signs of renal disease, fibrosis of glomeruli was observed; whereas in younger mice and those with milder signs of disease, focal and lobular glomerular changes were common.
Immunofluorescent staining revealed the deposition of large immunoglobulin complexes in the glomeruli of Nrf2–/– compared with much smaller or no complexes in Nrf2+/+ mice (Figure 5
, compare a and b); the immunoglobulines detected in the complexes included IgG (Figure 5)
, IgA, and IgM (data not shown). Similarly, deposition of complement C3 in glomeruli was markedly increased in Nrf2–/– mice in comparison with the controls (Figure 5
, compare c and d), indicating immune complex-mediated inflammatory responses in glomerulomembranes. Electron microscopic examination of kidney sections revealed predominantly proliferative changes with expansion of mesangial matrix and deposition of dense or amorphous material in diverse glomerular locations, including intramembranous, subendothelial, and mesangial sites (Figure 6, A and B)
. Loss (or fusion) of foot processes of podocytes was apparent in these kidneys. Together, the findings suggest increased deposition of immunoglobulins, complement activation in glomerular basement membranes, and proliferation of mesangial cells as contributing to membranoproliferative glomerulonephritis in Nrf2–/– mice.
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, which were indicative of renal failure and anemia resulting from severe glomerulonephritis.
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Initial necropsies of Nrf2–/– mice included histopathological examination of all tissues with gross lesions and unaffected major organs. As these necropsies were completed, an expanded spectrum of tissue changes became apparent in several mice, and additional tissues were sampled in subsequent necropsies, including all tissues with lesions and kidney, left lung lobe, heart, skin, spleen, thymus, pancreas, liver, bladder, inguinal lymph node, ileum, and mandibular salivary gland. In addition to glomerulonephritis, Nrf2–/– mice developed inflammatory lesions in multiple tissues, including lymphocytic sialitis (5 of 13 or 38%), dermatitis, hyperkeratosis, and/or epidermal clefting on the skin of the tail (which sometimes progressed to tail necrosis), myocarditis (8 of 31 or 26%), vasculitis (4 of 32 or 12%), and pancreatitis (4 of 18 or 22%). Two of the pancreatitis cases were lymphocytic pancreatitis, whereas two other cases were considered secondary to chronic-active vasculitis (one case of chronic-active, necrotizing pancreatitis and one case of proliferative pancreatitis associated with lymphoplasmacytic vasculitis with luminal obliteration and fibrinoid necrosis of vessel walls). Pleuritis and pericarditis were also frequently observed but may have been attributable to the development of thoracic transudates in mice with hypoproteinemia due to protein loss through the damaged glomeruli. Lymphocytic infiltrates were not seen in the central nervous system nor were neurological abnormalities the cause of death in any of these mice (these are the subject of a separate report currently in preparation).
As shown in Figure 8A
, the salivary glands of Nrf2-null mice showed intense periductal lymphocyte infiltration, reminiscent of Sjogren’s syndrome, an autoimmune disease of salivary glands often associated with systemic lupus erythematosus (SLE) in humans. Although lymphocytic infiltrates are not uncommon in mice, the 38% prevalence of lymphocytic sialitis seen in Nrf2-null mice is remarkable. In Figure 8B
, myocardial vacuolar degeneration and fibrosis are demonstrated. Occular necropsies were not routinely conducted on mice in this study. However, an occular necropsy of a representative Nrf2-null mouse with the occular discharge common in this strain demonstrated conjunctivitis, which varied from suppurative and lymphocytic conjunctivitis in the lower eyelids to upper eyelid alterations, which were lymphogranulomatous to pyogranulomatous with intralesional spaces consistent with lipoid material and rupture of meibomian gland contents. Associated changes included minimal to mild lymphocytic adenititis of the left and right lacrimal gland and the left harderian gland.
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compared with b and d). Low levels of immunoglobulin deposition in the epidermis of damaged skin were observed (Figure 9, e and f)
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The broad range of multitissue inflammatory lesions, along with glomerulonephritis and immunoglobulin deposition in blood vessels observed in Nrf2–/– mice, resembles the pathological characteristics of systemic lupus erythematosus (lupus) in humans, thus suggesting a role for Nrf2 in preventing the development of the autoimmune disease.
Spontaneous Development of Autoantibodies and Increased T-Cell Proliferation
A hallmark of lupus is the appearance of anti-dsDNA autoantibodies in blood. Nrf2–/– and age-matched control mice were examined for anti-dsDNA antibodies using ELISA. Serum anti-dsDNA antibodies were significantly elevated in Nrf2–/– mice in comparison with those of the homozygous and heterozygous control mice with the same 129SVJ background as well as C57BL/6 mice (Figure 10)
(P < 0.0001). The means of anti-dsDNA in Nrf2–/– mice were in the range of 1.0 to 2.1, whereas those of the control mice were from 0.14 to 0.32. In addition, the anti-dsDNA titers in female Nrf2–/– mice were twice as high as those of male Nrf2–/– mice, which was in agreement with a higher prevalence and greater severity of the immune-mediated diseases in females than in males.
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shows that T cells from Nrf2–/– mice exhibited enhanced proliferation on stimulation with anti-CD3 (a T-cell stimulant) in comparison with controls (P < 0.01). To further examine which subset of T cells accounted for the proliferation, CD4+ and CD8+ cells were isolated. The CD4+ cells from Nrf2–/– mice were shown to have increased proliferation in response to anti-CD3 (P < 0.05) (Figure 11B)
, whereas CD8+ cells from Nrf2–/– and Nrf2+/+ cells proliferated similarly under the same conditions (data not shown). B cells were isolated from the spleens of Nrf2+/+ and Nrf2–/– mice and were examined for proliferation in response to lipopolysaccharide or anti-mouse IgM (both stimulants of B-cell proliferation). The results revealed that B cells from Nrf2 wild-type and -null mice proliferate similarly to each other in response to the B-cell stimulants (data not shown). The compositions of peripheral CD4+ and CD8+ cells were analyzed by FACS. CD4+ and CD8+ cells each accounted for 20% of lymph node cells in Nrf2+/+ mice. However, in Nrf2–/– mice, the fraction of CD4+ cells was increased compared with controls (30 versus 20%), whereas that of CD8+ was reduced (14 versus 20%) (Figure 12)
. Taken together, these results suggest that loss of Nrf2 function is associated with an altered balance between peripheral CD4+ and CD8+ lymphocytes, which contributed to the development of immune-mediated disease in the mice. Hyperproliferation of T cells may also contribute to the adenopathy and splenomegaly observed in Nrf2-null mice (Figure 2C)
.
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Nrf2 is activated by a range of structurally diverse antioxidants, typified by phenolic antioxidants BHA and tBHQ. In wild-type mice, BHA induces two sets of genes: 1) phase II drug-metabolizing enzymes, such as Nqo1 and GstA1, and 2) antioxidant genes, such as Ho-1. The role of Nrf2 in the transcriptional regulation of these genes remains largely to be established. The high incidence of autoimmunity and enhanced lymphocyte proliferation in Nrf2-null mice raised the possibility that certain target genes of Nrf2 play critical roles in the control of self-tolerance, ie, loss of expression/induction of the genes contributes to immune disregulation. Thus, we examined the Nrf2 dependence in the expression of a panel of BHA-inducible genes in Nrf2-null mice. Female wild-type and Nrf2-null mice were treated with BHA or corn oil. Induction of the genes was analyzed by Northern blotting. As shown in Figure 13A
, phase II genes Nqo1, GstA1, UDP glucuronosyltransferase A1 (UgtA1), and epoxide hydrolase 1 (Ephx1) were constitutively expressed in the liver and were induced by BHA in wild-type mice; however, in Nrf2-null mice, induction of the genes, as well as the constitutive expression of Nqo1 and GstA1, was lost. Phase II genes Ephx2 and N-acetyltransferase 2 were expressed similarly in both wild-type and Nrf2-null mice in the absence or presence of BHA. Ho-1 and glutathione synthetase-S (Gsh-S) were induced by BHA in wild-type mice, but the induction was reduced or lost in Nrf2–/– mice. Thus, the Nrf2-null mice are devoid of the basal expression of Nqo1 and GstA1 as well as the induction of phase II genes (Nqo1, GstA1, UgtA1, and Ephx1) and antioxidative genes (Ho-1 and Gsh-S). We further examined whether Nrf2-null function affects the regulation of the ARE-driven genes in lymphoid tissues. Total RNA from the spleens of Nrf2+/+ and Nrf2–/– mice treated with BHA or corn oil was analyzed for expression of Nqo1 and Ho-1 by real-time PCR (Figure 13, B and C)
. The mRNAs of both genes were readily detected constitutively, but the levels were reduced in Nrf2–/– mice. Both were significantly induced by BHA in wild-type mice but not in null mice. Thus, Nrf2 controls the basal and inducible expression of Nqo1 and Ho-1 in splenocytes similarly to that in hepatocytes in vivo.
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and the kidney (Figure 14B)
of the Nrf2-null mice in comparison with those of wild-type mice (P < 0.05). In Figure 14C
, MDA production in the liver was shown to increase age-dependently in both genotypes. At the age of 1 month, the MDA contents were slightly higher in Nrf2–/– mice than in the wild-type. The differences were significantly increased at the ages of 5.5 and 11.5 months. The results indicate that Nrf2-null mice exhibited increased oxidative tissue damage in the absence of exposure to exogenous oxidants and suggest a synergistic effect on oxidative damage between Nrf2-null function and aging.
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Discussion |
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Several characteristics of the autoimmune-mediated lesions observed in the Nrf2–/– mice were similar to those of the human systemic lupus erythematosus. These include 1) erythematous skin lesions, membranoproliferative glomerulonephritis, serosities, and lymphocytic sialitis; 2) high levels of anti-dsDNA antibodies with renal deposition of immune complexes; 3) female predominance; and 4) variable courses of development. Interestingly, Yoh et al reported increased incidence of immune-mediated nephritis in a separate strain (ICR) of Nrf2-deficient mice.22 The immune-mediated glomer-ulonephritis in the ICR strain was also predominantly observed in females but at an older age (>60 weeks of age). The cause of the apparent age difference of the immune-mediated glomerulonephritis in Nrf2-deficient mice between the report by Yoh et al and our report is not known at present but may be attributable to differences in the genetic backgrounds of the two strains (ie, ICR versus 129SVJ). Nonetheless, the studies concur that loss of Nrf2 function predisposed mice to the development of lupus-like, systemic immune-mediated disease, principally characterized by membranoproliferative glomerulonephritis. Also consistent with SLE in humans, IgG, IgM, IgA, and C3 were all found in glomerular capillary deposits. Interestingly, dense deposits were predominantly intramembranous in Nrf2–/– mice. In addition, subendothelial and intramembranous deposits of amorphous material with varying electron density were observed in the glomeruli of Nrf2–/– mice. The most consistent light and electron microscopic finding in the glomeruli of Nrf2–/– mice was proliferation, predominantly of mesangial cells. In contrast to the previous report of glomerulonephritis,22 electron-dense deposits were not common in wild-type mice and, in fact, were seen in only one mouse in this series. Thus, our finding suggests that the absence of Nrf2 plays a role in the initiation of autoimmune disease rather than in its progression. As in human SLE, mesangial proliferation is a prominent feature of glomerulonephritis in these mice.
The development of SLE involves polyclonal activation of T and B lymphocytes, production of autoantibodies against nuclear and cytoplasmic macromolecules, and deposition of immune complexes in tissues, followed by a cascade(s) of inflammatory responses resulting in tissue damage.23,24
Evidence reveals that a complex interlay of genetic, environmental, and hormonal factors modulates these pathogenic mechanisms and thereby determine the manifestation, severity, and course of the disease.24,25
In particular, analyses of several experimental mouse models with spontaneous lupus-like syndromes have led to the identification of a number of candidate susceptibility genes of SLE, including class II major histocompatibility complex, complements, and immunoglobulin 
receptors IIa and IIIa. Furthermore, targeted disruption of certain genes or creation of transgenic strains with aberrant/overexpression of immune regulatory pathways have generated a collection of models of autoimmunity resembling SLE. Analyses of the models have not only revealed a large number of regulatory factors of SLE but also provided mechanistic insights into the effector mechanism involved in disease pathogenesis, the genetic mechanism leading to systemic autoimmunity, and the genetic interactions among susceptibility factors. It is noteworthy that enhanced proliferation of lymphocytes and elevated production of autoantibodies are common components of the systemic autoimmune syndromes observed in these mouse models. In our analysis of lymphocyte functions of Nrf2–/– mice, we found that peripheral CD4+ but not CD8+ T cells showed significantly enhanced proliferative response to anti-CD3 antibodies, a T-cell stimulant, giving rise to an increased ratio of CD4+ to CD8+ cells. On the other hand, B cells from Nrf2–/– spleens proliferate similarly to Nrf2+/+ cells on exposure to B-cell stimulants. It is known that the loss of anergy of anti-dsDNA B cells requires both the production of T helper cells and the overcoming of T suppressor cells.26
Therefore, our results implicate CD4+ hyperproliferation in the development of autoimmunity in Nrf2–/– mice. Nrf2 may negatively control CD4+ T-cell proliferation by inhibiting cell growth. Alternatively, Nrf2 regulates the sensitivity of CD4+ cells to growth stimulants by modulating the threshold of CD4+ cells to growth stimulants.
Analysis of a panel of phase II and antioxidant genes that are potentially regulated by AREs in Nrf2–/– females confirmed that Nrf2 is required for the induction of a number of ARE-regulated genes by antioxidants in both hepatic and lymphoid tissues (Figure 13)
. Ablation of Nrf2 reduces or abolishes the induction of phase II genes Nqo1, GstA1, UgtA1, and Ephx1 and antioxidant genes Ho-1 and Gsh-S, as well as the basal expression of Nqo1 and GstA1. It is known that these genes are directly or indirectly involved in the homeostasis of ROS. Reduction or loss of the expression and induction of the genes would result in increased oxidative stress in tissues. Increased lipid peroxidation (as indicated by elevated free MDA levels) is observed in the kidney, liver, and other tissues of Nrf2–/– mice. Furthermore, our data revealed a synergy between Nrf2-null function and aging on MDA production in vivo (Figure 14)
. This notion is supported by other reports in which real-time electron paramagnetic resonance imaging and spin probe kinetic analysis were used to examine the tissue-reducing activity of Nrf2–/– mice; the results indicated that Nrf2 deficiency plus aging significantly reduces the reducing capability in certain tissues of ICR mice.27
Together, these data provide direct evidence supporting a critical role of Nrf2 in the control of ROS homeostasis in intact animals.
Three lines of observation implicate oxidative stress in the loss of self-tolerance. First, exposure of lymphocytes to ROS, in particular H2O2, can mimic the effect of antigen exposure, leading to lymphocyte activation and proliferation. Moreover, antigen receptors are themselves H2O2-generating enzymes, raising the possibility of H2O2 as a second messenger in lymphocyte activation.28
Second, targeted knockout or certain polymorphisms of antioxidant genes, including target genes of Nrf2, were associated with immune-mediated nephritis.29,30
Third, supplementation of 
-3 fatty acids (as an antioxidant) up-regulated the expression of antioxidant enzymes (catalase, glutathione peroxidase, and superoxide dismutase) and delayed the onset and progression of autoimmune nephritis, thereby extending the life-span of lupus-prone NZB/NZW F1 female mice significantly.31
The correlation of impaired ROS homeostasis and autoimmune dysfunction observed in Nrf2-null mice supports a role of oxidative stress in lupus-like autoimmune regulation. It is known that loss of Nrf2 results in increased apoptosis due to increased ROS.16,32
Moreover, phagocytosis and clearance of apoptotic cells by macrophages have been linked to exposure of autoantigens to immune cells in the production of autoantibodies.33
Thus, our results provide a straightforward model to explain the breakdown in peripheral tolerance in Nrf2–/– mice: loss of Nrf2 causes oxidative tissue damage and apoptosis, which increase the production and exposure of autoantigens to immune cells, resulting in the activation of CD4+ cells and production of autoantibodies by B cells, leading to systemic autoimmune damage.
An alternative explanation of the autoimmune dysfunction in Nrf2–/– mice derives from the observation that the loss of function of certain drug-metabolizing enzymes (by targeted knockout or due to certain polymorphic genotypes) is associated with increased autoimmunity.30,34,35 In this scenario, altered metabolism of an endogenous or dietary chemical(s) in Nrf2–/– animals due to decreased expression of phase II enzymes may lead to increased production of reactive intermediates (other than ROS) that form haptens or directly damage macromolecules and cellular structures, both of which increase autoantigen production and activation of immune cells causing autoimmune response to self-tissues.
A prominent feature of lupus-like autoimmune syndromes is that many of the disorders can be induced or precipitated by drugs, pesticides, cosmetics, heavy metals, and other environmental, dietary, and occupational chemicals, thus underlining the importance of gene-environment interaction in autoimmune pathogenesis.36-40 Although it is unclear at present whether Nrf2 and its downstream enzymes are involved in chemical-induced autoimmune disorders, the critical role of Nrf2-regulated enzymes in the detoxification of a wide range of chemicals and the high inducibility of the enzymes by a variety of chemicals with diverse structures support such a role of Nrf2. In this regard, the Nrf2-null mice may provide a model system for analyzing possible interplay among lupus-inducing chemicals, drug metabolism, ROS generation, autoantibody production, and downstream pathogenic mechanisms in drug/toxicant-induced autoimmune dysfunctions in future.
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Footnotes |
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The findings and conclusions in this report are those of the authors and do not necessarily represent the views of the National Institute of Occupational Safety and Health.
Accepted for publication March 13, 2006.
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, Nrf2+/+; 
, Nrf2–/–. Data represent means ± SD from three samples. *P < 0.05.
