effects of chronic ochratoxin a exposure on p53 heterozygous and p53 homozygous mice
TRANSCRIPT
Effects of Chronic Ochratoxin A Exposure on p53 Heterozygousand p53 Homozygous Mice
GENEVIEVE S. BONDY1, DONALD S. CALDWELL
1, SYED A. AZIZ1, LAURIE C. COADY
1, CHERYL L. ARMSTRONG1,
IVAN H. A. CURRAN1, ROBYN L. KOFFMAN
2, KAMLA KAPAL1, DAVID E. LEFEBVRE
1, AND REKHA MEHTA1
1Food Directorate, Health Products and Food Branch, Health Canada, Ottawa, ON, Canada2Regions and Programs Bureau, Health Canada, Burnaby, BC, Canada
ABSTRACT
Exposure to the mycotoxin ochratoxin A (OTA) causes nephropathy in domestic animals and rodents and renal tumors in rodents and
poultry. Humans are exposed to OTA by consuming foods made with contaminated cereal grains and other commodities. Management of
human health risks due to OTA exposure depends, in part, on establishing a mode of action (MOA) for OTA carcinogenesis. To further inves-
tigate OTA’s MOA, p53 heterozygous (p53þ/�) and p53 homozygous (p53þ/þ) mice were exposed to OTA in diet for 26 weeks. The former
are susceptible to tumorigenesis upon chronic exposure to genotoxic carcinogens. OTA-induced renal damage but no tumors were observed in
either strain, indicating that p53 heterozygosity conferred little additional sensitivity to OTA. Renal changes included dose-dependent
increases in cellular proliferation, apoptosis, karyomegaly, and tubular degeneration in proximal tubules, which were consistent with ochra-
toxicosis. The lowest observed effect level for renal changes in p53þ/� and p53þ/þ mice was 200 mg OTA/kg bw/day. Based on the lack of
tumors and the severity of renal and body weight changes at a maximum tolerated dose, the results were interpreted as suggestive of a pri-
marily nongenotoxic (epigenetic) MOA for OTA carcinogenesis in this mouse model.
Keywords: ochratoxin; p53; mouse; carcinogenicity; chronic toxicity.
INTRODUCTION
Ochratoxin A (OTA) was first identified and structurally
characterized from a culture of Aspergillus ochraceus Wilh.
isolated from sorghum (van der Merwe et al. 1965) and is now
known to be produced by species in the fungal genera Aspergil-
lus and Penicillium (Varga et al. 2001). It is a phenylalanyl
derivative of a substituted isocoumarin (R)-N-[5-chloro-3,4-
dihydro-8-hydroxy-3-methyl-1-oxo-1H-2-benzopyran-7-y1)-
carbonyl]-L-phenylalanine (Marin et al. 2013, van der Merwe
et al. 1965). Although ochratoxigenic fungi may be present
on crops at harvest, OTA is primarily produced in storage when
crop moisture content, temperature, and other environmental
conditions favor fungal growth (Ominski et al. 1994). OTA is
widely distributed in food commodities including cereal grains,
dried fruits, and spices, coffee, beer, wine, cocoa, and meats
(Marin et al. 2013). Relative to other foods, consumption of
OTA in cereal grain–based foods contributes significantly to
human dietary OTA exposure (Duarte, Pena, and Lino 2010;
Kuiper-Goodman et al. 2010).
Exposure to OTA is nephrotoxic in rodents, pigs, and poul-
try, and causes renal tumors in rodents and poultry (Battacone,
Nudda, and Pulina 2010; Bendele et al. 1985; Boorman et al.
1992; Krogh et al. 1979; Stoev 2010). Thus, OTA has long
been a suspected contributor to human nephropathies. Expo-
sure to OTA in food has been linked to Balkan endemic
nephropathy (BEN), a chronic progressive renal disease associ-
ated with upper urothelial tract tumors that occur in rural popu-
lations along the Danube River (Pfohl-Leszkowicz 2009). In
this case, OTA involvement is controversial and there is also
evidence supporting the carcinogenic plant toxin aristolochic
acid as a causative agent of BEN (Grollman et al. 2007; Stefa-
novic, Polenakovic, and Toncheva 2011; Wu and Wang 2013).
A recent review of studies linking OTA to human nephropa-
thies concluded that there was no statistically significant evi-
dence for human health risks associated with OTA exposure.
However, the analysis was based on three studies that met the
established criteria for review, underscoring the need identified
by the authors for larger cohort or case-control OTA
The author(s) declared no potential conflicts of interest with respect to the
research, authorship, and/or publication of this article.
The author(s) received no financial support for the research, authorship,
and/or publication of this article.
Address correspondence to: Genevieve Bondy, Toxicology Research
Division 2202D, Bureau of Chemical Safety, Food Directorate, Health
Products and Food Branch, Health Canada, Ottawa, ON, Canada K1A 0K9;
e-mail: [email protected].
Abbreviations: AFIP, Armed Forces Institute of Pathology; ANOVA,
analysis of variance; BEN, Balkan endemic nephropathy; BW, body weight;
CLU, clusterin; D-PBS, Dulbecco’s phosphate buffered saline; DSB, double
strand break; ECP, eosinophilic crystalline pneumonia; EDTA,
ethylenediaminetetraacetic acid; ELISA, enzyme-linked immunosorbant
assays; EFSA, European Food Safety Authority; HR, homologous
recombination; 8-OHdG, 8-hydroxy-20-deoxyguanosine; IARC, International
Agency for Research on Cancer; Ig, immunoglobulin; JECFA, Expert
Committee on Food Additives; LOEL, lowest observed effect level; MOA,
mode of action; NIEHS, National Institute of Environmental Health
Sciences; NTP, National Toxicology Program; OPN, osteopontin; OSOM,
outer stripe of the outer medulla; OTA, ochratoxin A; p53þ/�, p53
heterozygous; p53þ/þ, p53 homozygous; PBS, phosphate buffered saline
solution; PCNA, proliferating cell nuclear antigen; PE-Cy5.5, phycoerythrin-
cyanine 5.5; PWM, pokeweed mitogen; TUNEL, terminal deoxynucleotidyl
transferase dUTP nick end labeling; WHO, World Health Organization.
1
Toxicologic Pathology, XX: 1-15, 2015
Copyright # 2015 by The Author(s)
ISSN: 0192-6233 print / 1533-1601 online
DOI: 10.1177/0192623314568391
epidemiology studies and for studies validating biomarkers of
human OTA exposure (Bui-Klimke and Wu 2014). Taken
together, the classification of OTA by the International Agency
for Research on Cancer (IARC) as a possible human carcino-
gen with sufficient evidence for carcinogenicity in experimen-
tal animals but inadequate evidence in humans (IARC 1993) is
consistent with current knowledge. Although nephropathy is
the primary noncancer outcome in OTA-exposed animals,
establishing a link between chronic kidney disease and OTA
exposure in humans is complicated by the multifactorial nature
of renal disease (Jha et al. 2013; McClellan and Flanders 2003)
and the lack of knowledge on OTA’s exact MOA.
Multiple MOAs for OTA-induced renal tumor formation
and nephropathy have been proposed based on in vivo and in
vitro studies. Although OTA exposure leads to DNA damage,
there is controversy about whether this occurs due to direct
interaction with DNA by OTA or a reactive OTA metabolite
(genotoxicity), or indirectly due to interaction of OTA or a
metabolite with non-DNA targets (nongenotoxicity). A cova-
lent DNA adduct (C-C8 OTA 30 dGMP) with mutagenic poten-
tial has been detected in kidneys from rats exposed to OTA,
although independent laboratories have not confirmed these
findings (Delatour et al. 2008; Mantle et al. 2010; Sharma,
Manderville, and Wetmore 2013). In support of an indirect
MOA, in vivo and in vitro studies indicate that OTA exposure
increases the production of reactive oxygen species (ROS)
leading to oxidative DNA damage in renal cells (Marin-Kuan
et al. 2011). There is also evidence that OTA disrupts antioxi-
dant defense responses regulated by the transcription factor
nuclear factor-erythroid 2-related factor 2 (Marin-Kuan et al.
2006), which could exacerbate ROS-induced oxidative stress
in kidney proximal tubule cells. Inhibition of gap junction
intercellular communication has been associated with cancer
development and has been shown to be disrupted by OTA in
vitro (Mally et al. 2006). Cell-based assays and transcriptomic
analyses of renal tissues and cultured cells indicate that OTA
can perturb posttranslational protein modifications that regu-
late many cellular functions (Jennings et al. 2012). These
include histone acetyltransferase inhibition leading to mitotic
disruption that may explain, in part, OTA-associated karyome-
galy, genetic instability, and tumorigenesis (Czakai et al. 2011;
Mally 2012).
Uncertainty in the MOA for OTA-induced DNA damage
impacts its risk assessment and management. Approaches for
food-borne carcinogens are based, in part, on the assumption
that there is no threshold for the dose response to genotoxic car-
cinogens, whereas homeostatic mechanisms impart a threshold
to the dose response elicited by nongenotoxic carcinogens
(Barlow et al. 2006). The Joint FAO/World Health Organiza-
tion (WHO) Expert Committee on Food Additives (JECFA)
considered that the weight of scientific evidence pointed
to multiple nongenotoxic MOAs for OTA (JECFA 2008).
Kuiper-Goodman et al. (2010) considered the genotoxicity of
OTA to be equivocal and based their health risk assessment
on genotoxicity, which is a default position for a substance with
an unknown carcinogenic MOA and not an acknowledgment
that genotoxicity per se is the MOA (European Food Safety
Authority [EFSA] 2005). While many in vitro and in vivo stud-
ies contribute to determining OTA’s MOA, multidose chronic
exposure and carcinogenesis studies provide the most valuable
dose–response data for risk assessment. Two-year carcinogen-
esis studies using F344/N and B6C3F1 mice are key studies for
OTA risk assessment (Bendele et al. 1985; JECFA 2008;
Kuiper-Goodman et al. 2010; NTP 1989). The present 26-
week study, a comparison of heterozygous p53þ/� mice and
corresponding p53þ/þ mice exposed to OTA in diet, provides
further data on the chronic toxicity and carcinogenicity of OTA
over a dose range relevant for risk assessment.
Transgenic mice heterozygous for a null p53 allele display
increased susceptibility to a wide range of carcinogens and a
low spontaneous tumor incidence rate up to about 9 months
in age (French, Storer, and Donehower 2001b). They have been
used as a model to identify potential chemical carcinogens
(Donehower et al. 1992; French et al. 2001a). The p53 protein
acts as a transcription factor that regulates multiple genes
involved in cellular functions and genome maintenance (Harris
and Levine 2005). The U.S. National Institute of Environmen-
tal Health Sciences/National Toxicology Program (NTP) eval-
uated the p53þ/� mouse for use in short-term carcinogenicity
testing and observed decreased latency and increased suscept-
ibility to tumor formation by genotoxic carcinogens (Dunnick
et al. 1997; French et al. 2001a; French, Storer, and Donehower
2001b; Pritchard et al. 2003; Tennant, Spalding, and French
1996). Previous chronic dietary exposure studies using the
p53þ/� mouse in our laboratory supported a nongenotoxic
MOA for the carcinogenic fungal toxin fumonisin B1, which
was consistent with the disruption of sphingolipid metabolism
and cellular regulators of apoptosis and proliferation rather
than direct genotoxicity (Bondy et al. 2012). In this study, the
p53þ/� mouse model was used to provide further insight into
the MOA for OTA carcinogenesis.
METHODS AND MATERIALS
Toxin and Diet Preparation
OTA (>98% purity; benzene free) was purchased from
Sigma-Aldrich Canada (Oakville, ON, Canada). All mice
received a modified AIN-93M diet (Dyets Inc., Bethlehem,
PA) during the acclimation period and throughout the study.
To prepare test diets, OTA was dissolved in methanol and
added to the diet. The resulting slurry was mixed thoroughly
while the methanol was removed by evaporation to dryness,
resulting in a stock diet containing 1.6 g of OTA/kg diet. The
OTA stock diet was mixed with control diet using an industrial
food mixer to prepare test diets containing 1-, 15-, or 40-mg
OTA/kg diet (weeks 1 and 2) and 0.5-, 2-, or 10-mg OTA/kg
diet (weeks 3–26).
Diet samples were collected monthly during the study to
verify OTA levels in treatment diets and to detect background
OTA levels in the control diet. Feed analyses methods were
adapted from Lombaert et al. (2003). Briefly, feed samples
were extracted with acetonitrile, methanol, and water (1:1:2)
2 BONDY ET AL. TOXICOLOGIC PATHOLOGY
by volume; centrifuged; and filtered. Aliquots of each sample
were diluted with phosphate buffered saline solution (PBS) and
cleaned up using an LCTech OTAClean immunoaffinity col-
umn (Dorfen, Germany) prior to OTA determination by liquid
chromatography (LC) with fluorescence detection. A 50-ml
volume was injected onto the LC system consisting of a Waters
Alliance 2695 liquid chromatograph (Milford, MA) combined
with Waters 2475 multiwavelength fluorescence detector and a
150 mm� 2.1 mm (3 mm) reversed phase Waters Atlantis dc18
analytical column. The fluorescence detector was set to 333 nm
excitation and 460 nm emission wavelengths.
The OTA primary reference standard (Sigma-Aldrich
Canada, Oakville, Ontario, Canada) was prepared in ben-
zene:acetic acid (99:1). Calibration standard solutions were
prepared in acetonitrile/water/acetic acid (99:99:2) by volume
ranging from 1 to 20 ng/ml, representing 2 to 40 ng/g in sam-
ples. The limit of quantitation for OTA was 6 ng/g. This was
determined as that level of standard in sample matrix producing
a chromatographic signal/noiseptp ratio of 10. The limit of
detection for OTA was 1.6 ng/g, determined with a chromato-
graphic signal/noiseptp ratio of 3.
Recovery experiments were performed with each sample set
using a known negative rodent feed sample. Samples were
spiked at 4 ng/g. The mean recovery for OTA was 108% (SD
¼ 2.5%, n¼ 3). Qualitative confirmation of the analyte identity
was performed by methyl esterification. Following sample
analysis, an aliquot of each calibration standard and sample
solution was removed and methyl esterified. Methyl esterifica-
tion resulted in the diminution of the OTA chromatographic
peak and the appearance of a new chromatographic peak corre-
sponding to methyl-OTA.
Animals and Study Design
Forty male p53þ/� mice (P53N5-T) mice and 40 male
p53þ/þ (P53N5-W) mice, 5 to 7 weeks old, were purchased
from Taconic Farms Inc. (Germantown, NY). Mice were
weighed and individually caged upon arrival. Cages were
housed in semirigid HEPA-filtered isolator units manufactured
for Health Canada by Charles River (Boston, MA). Mice
received modified AIN-93M diet and water ad libitum for 1
week prior to the study while acclimating to the animal facility
and isolator units. Temperature and humidity inside the isolator
units were monitored daily for the duration of the study.
Throughout the study, mice received care and handling accord-
ing to the requirements of the Canadian Council for Animal
Care.
The mean body weight (BW) of all mice (p53þ/þ and
p53þ/�) upon arrival was 26.0 + 2.4 g. During acclimation,
p53þ/þ and p53þ/� mice were divided randomly into 4
groups of 10 mice/dose/strain. There were no significant differ-
ences in starting BWs across dose groups and strain at the
beginning of the study (Table 1). During the study, mice
received water and control or test diet ad libitum. BW and food
consumption data were collected weekly. At the beginning of
the study, p53þ/þ and p53þ/� mice received feed containing
0-, 1-, 15-, or 40-mg OTA/kg diet, as in Bendele et al. (1985).
By the end of week 2, BWs in p53þ/þ mice were 20% and
28% lower in the 15- and 40-mg/kg dose groups, respectively;
in p53þ/�mice, BWs were 27% and 31% lower in the 15- and
40-mg/kg dose groups, respectively (Figure 1A and B). Due to
rapid weight loss, test diets were removed from the p53þ/þand p53þ/�medium- and high-dose groups at the end of week
2 and replaced with control diet for 24 hr. After 24 hr, reformu-
lated diets were given to all test groups (Figure 1). For the
remainder of the study, mice received 0-, 0.5-, 2-, or 10-mg
OTA/kg diet. After 26 weeks, final BWs were recorded and all
mice were exsanguinated by cardiac puncture under isoflurane
anesthesia (Baxter Corporation, Mississauga, ON, Canada).
Organ weights were recorded at necropsy for liver, kidney, thy-
mus, and spleen.
Hematology and Immunology
Whole blood was collected in ethylenediaminetetraacetic
acid (EDTA) at necropsy. White blood cells (WBCs), neutro-
phils, lymphocytes, monocytes, eosinophils, and basophils were
enumerated using a Coulter AcTTM 5 Diff Cap Pierce Hematol-
ogy Analyzer (Beckman Coulter, Mississauga, ON, Canada).
Immunophenotype analysis of whole blood by flow cyto-
metry was based on four color panels using the following
monoclonal antibodies (BD Biosciences, Mississauga, ON,
TABLE 1.—Initial BW, final BW, and final organ weights of p53þ/þ and p53þ/� mice exposed to dietary OTA for 26 weeks.
p53þ/þ p53þ/�
OTA added to diet
(mg OTA /kg diet)a 0 0.5 2 10 0 0.5 2 10
Initial BW (g) 28.8 + 3.9 28.4 + 3.0 30.2 + 3.3 30.3 + 2.6 28.7 + 3.1 29.3 + 2.5 28.4 + 1.7 28.2 + 1.8
Final BW (g) 48.0 + 4.9 46.5 + 3.3 42.4 + 4.4b 33.5 + 3.9b 45.7 + 3.5 46.8 + 3.1 39.4 + 2.7b 28.6 + 2.9b
Liver (% BW) 5.95 + 0.85 5.37 + 0.48 4.59 + 0.51b 4.37 + 0.34b 5.52 + 0.84 5.47 + 0.43 4.46 + 0.42b 4.27 + 0.24b
Kidney (% BW) 0.43 + 0.04 0.42 + 0.03 0.40 + 0.05 0.35 + 0.02b 0.41 + 0.02 0.40 + 0.02 0.40 + 0.02 0.37 + 0.02b
Spleen (% BW) 0.23 + 0.02 0.23 + 0.05 0.23 + 0.02 0.28 + 0.04b 0.20 + 0.02 0.21 + 0.03 0.21 + 0.01 0.27 + 0.03b
Thymus (% BW) 0.09 + 0.02 0.08 + 0.02 0.08 + 0.01 0.10 + 0.01 0.08 + 0.01 0.09 + 0.02 0.09 + 0.02 0.11 + 0.02b
Note: OTA ¼ ochratoxin A; BW ¼ body weight.aDietary OTA levels for week 3 to 26. bData are significantly different from corresponding controls using analysis of variance (ANOVA) followed by post hoc pairwise comparisons
using the Holm–Sidak or Dunn’s test (p � .05).
Vol. XX, No. X, 2015 OCHRATOXIN A EFFECTS ON P53þ/� MICE 3
Canada): rat anti-mouse CD45 phycoerythrin-cyanine 5.5 (PE-
Cy5.5) clone 30-F11, Leucocyte Common Antigen; hamster
anti-mouse CD3e fluorescein isothiocyanate clone 145-2C11,
T lymphocyte; rat anti-mouse CD4 allophycocyanine clone
RM4-5, T helper lymphocyte; rat anti-mouse CD8a R-
phycoerytherin clone 53-6.7, T cytotoxic lymphocyte; rat
anti-mouse CD19 allophycocyanine clone 1D3, B lymphocyte;
rat anti-mouse CD49b phycoerythrin clone DX5, natural killer
cell. Blood samples were mixed with antibodies and incubated
for 10 min protected from light at room temperature. Red blood
cells were lysed using a TQ-Prep (Beckman Coulter, Missis-
sauga, ON, Canada) and Immunoprep lysis reagent (Beckman
Coulter, Brea, CA). Lymphocyte subset analyses were per-
formed by flow cytometry using a Becton Dickinson FACSCa-
libur System equipped with 488 nm and 635 nm air-cooled
lasers (BD Biosciences, Mississauga, ON, Canada).
Splenocyte suspensions for immunophenotyping were pre-
pared in Dulbecco’s phosphate buffered saline (D-PBS;
Gibco/Invitrogen, Grand Island, NY) by gently crushing tissues
in a 70-mm nylon cell strainer (BD Falcon, Bedford, MA) and
rinsing into a 50-ml tube. Prior to staining, WBCs were counted
using a Beckman Coulter AcTTM 5 Diff Cap Pierce Hematology
Analyzer and cell suspensions were standardized to 2 � 107
WBCs/ml. Cell staining was performed by mixing a 100 mL
aliquot of suspended splenocytes with antibodies as described
previously and fixing using 0.1% buffered formaldehyde.
Splenocytes for proliferation assays were released from the
spleen by gentle dispersion into D-PBS using tissue forceps.
Erythrocytes were removed by lysis using ammonium-
chloride-potassium lysing buffer (Quality Biological Inc.,
Gaithersburg, MD), splenocytes were strained with trypan
blue, and viable cells were enumerated using a hemocytometer.
Cultures containing 5 � 105 viable splenocytes in Gibco serum-
free AIM-V medium supplemented with 2-mercaptoethanol
(Invitrogen Canada Inc., Burlington, ON, Canada) were incu-
bated in the presence of pokeweed mitogen (Sigma) or medium
only (unstimulated controls) for 72 hr. Splenocyte proliferation
was measured by quantifying 6-hr 3H-methylthymidine
(1 mCi/ well) incorporation using a LKB Wallac liquid scintil-
lation counter (Perkin Elmer Life Sciences, Woodbridge, ON,
Canada).
Total plasma immunoglobulin levels were analyzed by
sandwich enzyme-linked immunosorbant assays (ELISA)
using primary and secondary antibodies specific for mouse
IgA, IgG, and IgM (Bethyl Laboratories Inc., Montgomery,
TX). Sandwich ELISAs were performed according to the pro-
tocol accompanying the antibodies using buffers and reagents
as described by Tryphonas et al. (2004).
Histology
A gross visual examination was performed on each mouse at
necropsy. Liver, right kidney, thymus, spleen, esophagus, tra-
chea, thyroid, stomach (including forestomach), ileum (includ-
ing Peyer’s patches), mesenteric lymph nodes, popliteal lymph
nodes, heart, and lungs were fixed by immersion in 10% neutral
buffered formalin. Samples from the fixed tissues were paraffin
embedded and blocked. The tissue blocks were sectioned to 5
mm, stained with hematoxylin and eosin according to the
method described by Luna (1968), and examined by light micro-
scopy. Renal lesions were classified according to International
Harmonization of Nomenclature and Diagnostic Criteria nomen-
clature (Frazier et al. 2012). Lesion severity was graded subjec-
tively in comparison to control animals and assigned a numeric
score from 0 to 5 where 0 indicated that a lesion was not present
or present within subjective normal limits, and where 1 through
5 indicated that lesions were minimal, mild, moderate, marked,
and severe, respectively. Lymphoid tissues were assessed for
direct immunotoxicity according to International Collaborative
Immunotoxicity Study (1998). Testes were fixed by immersion
in Bouin’s fixative at necropsy. After 24 hr, they were washed
and transferred to 70% ethanol. Fixed testes were trimmed to
produce transverse sections at the level of rete and then
embedded in paraffin. Tissue blocks were sectioned to 5 mm and
stained with periodic acid Schiff hematoxylin. A section from
the right testes of each mouse was evaluated by light microscopy
for standard lesions (Foley 2001; Lanning et al. 2002).
Renal Immunohistochemistry
Unstained kidney sections (5 mm thick) were used for immu-
nohistochemical procedures. To detect proliferating cells, sec-
tions were first subjected to antigen retrieval by heating in 10
mmol/L sodium citrate buffer in a microwave for 2.5 min. The
mouse monoclonal anti-proliferating cell nuclear antigen
(PCNA) antibody (DakoCytomation, Carpinteria, CA), diluted
1:10,000, was used as the primary antibody. The EnVisionTM
þ System (DakoCytomation), using an anti-mouse secondary
antibody conjugated with horseradish peroxidase followed by
detection with diaminobenzidine, was applied according to the
manufacturer’s instructions to visualize PCNA-positive cells.
Harris’s hematoxylin was used as the counterstain.
For apoptosis, the ApopTag1 Plus Peroxidase In Situ Apop-
tosis Kit (Chemicon, Temecula, CA) was used according to the
manufacturer’s instructions. This terminal deoxynucleotidyl
transferase dUTP nick end labeling (TUNEL) assay-based
method detects early apoptosis via DNA fragmentation by enzy-
matically labeling the free 30-OH termini with modified nucleo-
tides. Briefly, sections were subjected to a protein digestion
enzyme to quench endogenous peroxidase, followed by applica-
tion of an equilibration buffer and incubation with TdT enzyme,
before stopping the reaction by adding anti-digoxigenin
FIGURE 1.—Time line for exposure of p53þ/þ and p53þ/� mice to
ochratoxin A in diet.
4 BONDY ET AL. TOXICOLOGIC PATHOLOGY
conjugate buffer. This was followed by incubation with the per-
oxidase substrate and counterstain with methyl green.
For clusterin (CLU) detection, sections were first subjected
to antigen retrieval by heating in Tris EDTA, pH 9, in a 100�Cwater bath for 30 min. Sections were incubated with the pri-
mary antibody rabbit polyclonal anti-CLU (Santa Cruz Bio-
technology, Dallas, TX) diluted 1:100, followed by detection
with the EnVisionTM þ System (DakoCytomation) and Har-
ris’s hematoxylin counterstain.
To detect osteopontin (OPN), kidney sections were first sub-
jected to antigen retrieval by heating in a commercially
obtained antigen retrieval solution (S1700; Dako Cytomation)
in a water bath at 100�C for 30 min. After blocking endogenous
biotin, biotin receptor, and avidin binding sites (Avidin/biotin
blocking kit, Vector Laboratories, Burlingame, CA), sections
were incubated with the primary antibody rabbit polyclonal
anti-OPN (Abcam Inc., Cambridge, MA) diluted 1:250, fol-
lowed by detection with the EnVisionTM þ System (Dako
Cytomation) and Harris’s hematoxylin as the counterstain.
The immunostained sections were analyzed using a Zeiss
Axiophot light microscope (Carl Zeiss Canada Ltd., Toronto,
ON, Canada) and image analysis. Proliferating (PCNA-posi-
tive) and apoptotic (TUNEL-positive) cells were enumerated
in proximal tubules for 1 entire kidney section per mouse. The
ratios of proliferating cells (PCNA-positive) or apoptotic cells
(TUNEL-positive) per section area (mm2) were determined
using Northern Eclipse Version 7.0 software (Empix Imaging,
Inc., Mississauga, ON, Canada). Semiquantitative assessments
were conducted on CLU- and OPN-stained sections. Ten fields
per section covering most of the section area were assessed for
percentage proximal tubule staining in each field using North-
ern Eclipse version 7.0 software, generating a mean percentage
positivity score for 1 kidney section per mouse.
Statistical Analyses
Statistical comparisons were conducted using SigmaPlot 12
(Systat Software, Inc., San Jose, CA). Data were analyzed for nor-
mality using the Kolmogorov–Smirnov test. Equal variance was
tested by checking the variability around group means. Within
each strain (p53þ/þ or p53þ/�), multiple group comparisons
were conducted by 1-way analysis of variance (1-way ANOVA),
followed by post hoc pairwise comparisons using the Holm–
Sidak test. Multiple group comparisons of nonparametric data
were conducted using the Kruskal–Wallis ANOVA on Ranks,
followed by post hoc pairwise comparisons using the Dunn’s
method. Animal weights and relative food consumption (food
consumption/BW) were analyzed by ANOVA on weekly average
weights (Hoffman, Ness, and van Lier 2002). For histopathology
endpoints, including CLU and OPN data, lesion severity data
were analyzed using the Kruskal–Wallis 1-way ANOVA on
Ranks within each strain. Comparisons of data from p53þ/þ and
p53þ/� mice were conducted by 2-way ANOVA to identify
interactions between strain and dose, followed by post hoc pair-
wise comparisons using the Holm–Sidak method.
RESULTS
Diet Analyses
OTA was not detected in control diets. Levels of OTA
detected in treatment diets are summarized in Tables 2 and 3.
After correcting for recovery, OTA was recovered from treat-
ment diets at levels 20–30% lower than OTA added to diets
at preparation.
Effects of OTA on BW, Food Consumption, and Organ
Weight
In the first 2 weeks on diet, BW gain in all mice in the medium
(15-mg OTA/kg diet) and high (40-mg OTA/kg diet) dose
groups was significantly depressed compared to mice in the con-
trol and low (1 mg/kg) dose groups. By the end of week 2, BWs
in p53þ/þmice were 20% and 28% lower in the 15- and 40-mg/
kg dose groups, respectively; in p53þ/� mice, BWs were 27%and 31% lower in the 15- and 40-mg/kg dose groups, respec-
tively (Figure 2A and B). It was decided that medium- and
high-dose group mice would not survive the 26-week exposure
period, so reformulated diets containing lower OTA levels were
introduced at the beginning of week 3. From this time onward,
mice in the new medium (2-mg OTA/kg diet) and high (10 mg
OTA/kg diet) dose groups gained weight. Control p53þ/þ and
p53þ/� mice and mice in the new low-dose group (0.5-mg
OTA/kg diet) gained weight throughout the exposure period.
In both p53þ/þ and p53þ/�mice, BWs of low-dose mice were
not significantly different from respective controls at any time
(Figure 2A and B). Mean BWs of medium-dose p53þ/þ mice
were significantly lower than respective controls in week 2 and
weeks 6–26. Mean BWs of high-dose p53þ/þ mice were
TABLE 2.—Ochratoxin A consumption by p53þ/þ and p53þ/� mice in week 1 of the 26-week exposure period.
p53þ/þ p53þ/�
OTA added to diet (mg OTA /kg diet) 0 1 15 40 0 1 15 40
OTA analyzed in diet (mg OTA/kg diet)a <4 � 10�4 0.8 10.2 31.7 <4 � 10�4 0.8 10.2 31.7
Mean daily OTA consumption based on
OTA recovered from diet (mg OTA/kg
BW/day)
0 0.12 + 0.02 1.44 + 0.49 4.42 + 1.52 0 0.09 + 0.01 1.30 + 0.23 3.94 + 1.21
Note: OTA ¼ ochratoxin A; BW ¼ body weight.aOne feed sample from week 1 for each diet/dose group was analyzed as described in the Methods and Materials section.
Vol. XX, No. X, 2015 OCHRATOXIN A EFFECTS ON P53þ/� MICE 5
significantly lower than respective controls from weeks 1 to 26
(Figure 2A). In p53þ/� mice, mean BWs of medium and high
dose mice were significantly lower than respective controls
from weeks 1 to 26 (Figure 2B).
The effect of OTA exposure on BW-normalized food con-
sumption (relative food consumption) was evaluated for each
week of the study (Figure 3A and B). In p53þ/þ medium-
dose mice, relative food consumption was significantly higher
than in respective controls from weeks 6 to 11; in p53þ/þhigh-dose mice, relative food consumption was significantly
higher than in respective controls in week 3 and weeks 4 to
26 (Figure 3A). In p53þ/� medium-dose mice, relative food
consumption was higher than in respective controls in weeks
3, 4, 6, 10, 11, 14 to 17, 19, and 21 to 23. In p53þ/� high-
dose mice, relative food consumption was significantly higher
than in respective controls from weeks 1 to 26 (Figure 3B).
Mean daily OTA consumption values were calculated based
on OTA levels detected in diets, food consumption, and BW
(Tables 2 and 3). In the 1st week of the study, mean daily OTA
consumption values were 0.12-, 1.44-, and 4.42-mg OTA/kg
bw/day for p53þ/þ low-, medium-, and high-dose diets,
respectively. For p53þ/� low-, medium- and high-dose
groups, mean daily OTA consumption values were 0.09-,
1.30-, and 3.94-mg OTA/kg bw/day, respectively. Calculations
were not possible for week 2 due to feed refusal and feed
wastage in the medium- and high-dose groups (Table 2); how-
ever, similar calculations were done for the remaining 24
weeks of the study (Table 3). Mean daily OTA consumption
increased over week 3 to 24, in parallel with increasing relative
food consumption. This resulted in a range of mean daily OTA
consumption values calculated for weeks 3 to 26 which were
lowest early in the study and gradually increased to the highest
value by the end of the study (Table 3).
Final organ weights expressed as percentage BW are sum-
marized in Table 1. Liver weights were significantly reduced
relative to respective controls in p53þ/þ and p53þ/� mice
in the medium- and high-dose groups, and kidney weights were
significantly reduced in p53þ/þ and p53þ/�mice at the high-
est dose. Spleen weights were significantly increased in p53þ/
þ and p53þ/� mice in the high-dose group. Relative thymus
weights were significantly higher relative to controls in
p53þ/� mice in the high-dose group.
Effects of OTA on Immune Parameters
There were no significant changes due to OTA in numbers
of circulating WBCs, lymphocytes, lymphocyte subsets, or
granulocytes (data not shown). There were no significant
changes in splenocyte subpopulations due to OTA exposure
(data not shown). Splenocyte proliferation was significantly
reduced in p53þ/þ mice in the high-dose group relative to
controls (Figure 4). Plasma total immunoglobulin M, G, and
A levels were unaffected by OTA in p53þ/þ and p53þ/�mice
(data not shown).
Histopathologic Changes in Mice Exposed to OTA
Hepatocytes were markedly enlarged with cytoplasmic
clearing and vacuolation in the livers of control and low-dose
mice of both strains, which was generally associated with
relatively high body fat levels. In medium-dose p53þ/þ and
p53þ/� mice, hepatocytes were less swollen with less
cytoplasmic clearing and vacuolation. In high-dose mice,
hepatocyte cytoplasmic swelling with vacuolation was not
observed. Occasional foci of hepatocellular necrosis were
observed in all control and low-dose mice. The incidence and
severity of focal necrosis increased in medium- and high-
dose mice relative to controls. There were no strain-related dif-
ferences in the incidence and severity of hepatocellular necro-
sis (data not shown).
The incidence and severity of renal lesions in p53þ/þ and
p53þ/� mice are summarized in Table 4 and examples of typ-
ical renal lesions are shown in Figure 5. In both strains, micro-
scopic lesions were evident in renal tissues at all doses,
dominated by increasingly severe and prevalent karyomegaly,
apoptosis, and anisokaryosis affecting the proximal tubular
epithelium, including the S1 and S2 convoluted segments (cor-
tical labyrinth) and the S3 straight segments (outer stripe of the
outer medulla [OSOM] and medullary ray). Rare epithelial
cells with mild degeneration were present in the tubular epithe-
lium in the 0.5-mg OTA/kg dose group in both mouse strains.
TABLE 3.—Ochratoxin A consumption by p53þ/þ and p53þ/� mice from week 3 to 26 of a 26-week exposure period.
p53þ/þ p53þ/�
OTA added to diet (mg OTA /kg diet) 0 0.5 2 10 0 0.5 2 10
OTA analyzed in diet (mg OTA/kg diet)a <4 � 10�4 0.39 + 0.05 1.47 + 0.23 7.81 + 0.39 <4 � 10�4 0.39 + 0.05 1.47 + 0.23 7.81 + 0.39
Mean daily OTA consumption values for week 3
to 26 based on OTA recovered from diet (mg/
kg bw/day)b
0 0.03 + 0.01 0.20 + 0.06 1.46 + 0.35 0 0.03 + 0.00 0.19 + 0.05 1.55 + 0.42
Range of calculated mean daily OTA
consumption values for week 3 to 26 (mg/kg
BW/day)c
0 0.04 – 0.07 0.18 – 0.44 1.50 – 2.41 0 0.04 – 0.05 0.20 – 0.45 1.61 – 3.01
Note: OTA ¼ ochratoxin A; BW ¼ body weight.aMonthly feed samples from each dose group, n ¼ 6 samples total/dose group, were analyzed as described in the Methods and Materials section. OTA was not detected in control
diet. bReliable food consumption values for week 2 were unavailable due to feed refusal and coincident feed wastage. cOTA consumption gradually increased over time as mice gained
weight and consumed correspondingly more diet.
6 BONDY ET AL. TOXICOLOGIC PATHOLOGY
Mild tubular degeneration, evident as cytoplasmic vacuolation
with or without pale basophilic coloration, was observed in the
2-mg OTA/kg dose group in both mouse strains. In the 10-mg
OTA/kg dose groups, occasional regenerative tubules were
observed in the cortex, with mild tubular degeneration affect-
ing cortical tubular epithelium. No adenomas, carcinomas, or
cystic tubules lined by hyperplastic epithelium, as described
by Bendele et al. (1985), were detected.
There were no lesions in immune tissues, including thymus,
Peyer’s patches, spleen, and mesenteric and inguinal lymph
nodes. Mild degenerative lesions were observed in testicular
seminiferous tubules from all mice. These changes appeared
to be more prevalent in p53þ/þ than in p53þ/� mice across
all doses, although this observation was not quantified.
There were no lesions in any other tissues examined, with
the exception of the lungs. In the lungs of p53þ/þ and
p53þ/� mice in all dose groups, including controls, lesions
consistent with eosinophilic crystalline pneumonia (ECP) were
observed (Hoenerhoff, Starost, and Ward 2006). In control,
low-, and medium-dose mice, these lesions were characterized
by mild to marked lymphoid/ plasma cell infiltration in peri-
bronchiolar and perivascular regions. Scattered in the alveoli
were few macrophages containing abundant densely eosinophi-
lic cytoplasm that had a crystalline appearance. Large eosino-
philic rod-shaped crystals occurred occasionally in bronchiolar
lumens. In high-dose mice, similar lesions appeared to be more
FIGURE 2.—Mean body weights (BWs; g; þSD) in (A) p53þ/þ and
(B) p53þ/� mice exposed to ochratoxin A in diet for 26 weeks. Mean
BWs of medium-dose p53þ/þ mice were significantly lower than
respective controls in week 2 and weeks 6 to 26; mean BWs of
high-dose p53þ/þ mice were significantly lower than respective con-
trols from weeks 1 to 26 (A). Mean BWs of medium-and high-dose
p53þ/� mice were significantly lower than respective controls from
weeks 1–26 (B).
FIGURE 3.—Mean weekly feed consumption (g; þSD) in (A) p53þ/þand (B) p53þ/�mice exposed to ochratoxin A in diet for 26 weeks. In
p53þ/þ medium-dose mice, relative food consumption was signifi-
cantly higher than in respective controls from weeks 6 to 11; in
p53þ/þ high-dose mice, relative food consumption was significantly
higher than in respective controls in week 3 and weeks 4 to 26 (A). In
p53þ/� medium-dose mice, relative food consumption was higher
than in respective controls in weeks 3, 4, 6, 10, 11, 14 to 17, 19, and
21 to 23. In p53þ/� high-dose mice, relative food consumption was
significantly higher than in respective controls from weeks 1 to 2 (B).
Vol. XX, No. X, 2015 OCHRATOXIN A EFFECTS ON P53þ/� MICE 7
severe. Figure 6 demonstrates a prominent needle-shaped crys-
tal visible in a bronchiole from a control p53þ/� mouse. The
diagnosis of ECP was verified by consultation with the Armed
Forces Institute of Pathology (AFIP 2008), although the
‘‘crystalline’’ component was not considered striking. A fur-
ther observation in the lungs of all mice, regardless of strain
and dose, was that of mild bronchiolar epithelial cell hyper-
plasia, mild smooth muscle hyperplasia of bronchioles and
prominent smooth muscle hyperplasia in the tunica media
of lung arterioles. The degree of smooth muscle hyperplasia
was similar across dose groups and strains. These lesions were
also verified by the AFIP (2008), and are not known to be
associated with ECP.
Immunohistochemical Assessment of Kidneys from OTA-
exposed Mice
Quantitative and semiquantitative immunohistochemical
assessments of kidney sections from p53þ/þ and p53þ/�mice are summarized in Table 5. A dose-dependent increase
in PCNA-positive epithelial cells in the proximal tubules of
p53þ/þ and p53þ/� mice was observed, which was signifi-
cantly greater in both strains exposed to 10-mg OTA/kg diet
compared to the corresponding controls. The number of apop-
totic epithelial cells was also significantly higher in proximal
tubules of p53þ/þ and p53þ/� mice in the 10-mg OTA/kg
dose group. Expression of the kidney injury biomarkers CLU
and OPN in proximal tubules was significantly increased
in p53þ/þ mice in the 10-mg OTA/kg dose group and in
p53þ/� mice in the 2- and 10-mg OTA/kg dose groups
(Table 5; Figure 7). CLU and OPN expression were also higher
with increasing OTA exposure in distal convoluted tubules
from p53þ/þ and p53þ/� mice, with the difference achieving
significance at the highest dose (data not shown).
Comparison of Changes in p53þ/þ and p53þ/� Mice
Differences in the responses of p53þ/� versus p53þ/þmice to OTA were not pronounced. Final BWs were 15% lower
in high-dose p53þ/�mice compared to p53þ/þmice; this dif-
ference was not statistically significant (Table 1). In compari-
son, final BWs were 5%, 0%, and 7% lower in p53þ/� mice
compared to p53þ/þ in the control-, low-, and medium-dose
groups (Table 1). Compared to their respective controls, signif-
icant differences in BW and relative food consumption
occurred more often in p53þ/� than p53þ/þ mice (Figure
2A and B; Figure 3A and B). There were significantly higher
numbers of apoptotic cells in proximal tubules of p53þ/�mice
exposed to 0.5-mg and 10-mg OTA in diet, respectively, com-
pared to p53þ/þ mice exposed to the same levels of OTA in
diet (Table 5). Although CLU and OPN expression were signif-
icantly higher in p53þ/� mice but not p53þ/þ mice exposed
to 2-mg OTA/kg diet, the apparent difference between strains
was not statistically significant. There were no further statisti-
cally significant strain-related differences in responses to OTA
for any other endpoint examined.
DISCUSSION
Hepatic and renal tumors were observed in male B6C3F1
mice exposed chronically to 40-mg OTA/kg diet (Bendele
et al. 1985; Kanisawa and Suzuki 1978). In this study, male
p53þ/þ and p53þ/� mice could not be fed diets containing
15- or 40-mg/kg OTA due to rapid and significant weight loss.
Mice were switched to new diets containing 0.5-, 2-, and 10-mg
OTA/kg diet to replace diets containing 1-, 15-, and 40-mg
OTA/kg diet, respectively. Feed consumption measurements
during the initial period were highly variable in the 15- and
40-mg/kg dose groups, primarily due to the mice removing diet
from feed containers. This activity, presumably motivated by
dissatisfaction with the diet, obscured any measurement of
putative changes in food consumption. However, even with
an assumption that BW changes were due to reduced feed con-
sumption, it could not be established whether feed refusal was
due to unpalatability or to OTA morbidity with concurrent
inappetance.
At the end of the study, a dose-dependent increase in hepa-
tocellular necrosis, but no tumors or preneoplastic lesions were
observed in the livers of p53þ/þ and p53þ/� mice. Likewise,
renal changes were consistent with OTA-induced nephrotoxi-
city, but no tumors were observed in the kidneys of p53þ/þand p53þ/� mice. It is possible that tumors may have devel-
oped if the exposure period had been longer or if it were
possible to use the higher dietary OTA levels that caused
tumors in B6C3F1 mice (Bendele et al. 1985). Validation of the
p53þ/� mouse model for carcinogenesis bioassays initially
indicated that a 26-week exposure period was sufficient for true
positive responses to develop in p53þ/�mice after exposure to
genotoxic compounds known to pose carcinogenic risks for
FIGURE 4.—Pokeweed mitogen (PWM)-stimulated proliferation in
splenocyte cultures from p53þ/þ and p53þ/� mice exposed to ochra-
toxin A in diet for 26 weeks. Proliferation is expressed as 3H-thymidine
incorporation (disintegrations per minute) in PWM-stimulated cul-
tures/3H-thymidine incorporation in unstimulated cultures. *Signifi-
cantly different from corresponding controls (p < .05).
8 BONDY ET AL. TOXICOLOGIC PATHOLOGY
humans (Floyd et al. 2002); however, exposure periods up to 9
months have been used with no increased mortality in control
animals (NTP 2005a, 2005b). In this study, it was assumed that
the maximum tolerable dose had been achieved at 10-mg OTA/
kg diet based on significant weight loss in mice initially
exposed to 15-mg OTA/kg diet. Furthermore, BW and liver
weight reduction in p53þ/� and p53þ/þ mice exposed to
10-mg OTA/kg diet were indicative of morbidity. Final BWs
were 30% and 37% lower, respectively, and relative liver
weights were 27% and 23% lower, respectively, in high-dose
p53þ/þ and p53þ/� mice in this dose group. In comparison,
BWs of B6C3F1 mice exposed to 40 ppm OTA in diet were
20% and 30% lower than those exposed to 0 ppm or 1 ppm
OTA in diet in months 6 to 24 of a 2-year study (Bendele
et al. 1985). This supports the conclusion that the absence of
tumors in p53þ/�mice in this study was not an artifact of dose
selection or exposure period. Since p53þ/� mice are sensitive
to genotoxic carcinogens, the lack of tumors and the overall
similarity in responses to OTA in p53þ/� and p53þ/þ mice
suggest that the MOA for OTA carcinogenesis is primarily
nongenotoxic.
Similar responses to OTA in p53þ/þ and p53þ/� mice
indicate that p53 heterozygosity did not strongly influence
renal toxicity, suggesting either a limited role for p53 and
p53-regulated pathways in response to OTA-induced cellular
toxicity or significant redundancy in cellular protective
mechanisms to compensate for p53 deficiency. The only statis-
tically significant difference between p53þ/� and p53þ/þmice was a higher number of apoptotic cells in kidney OSOM
in p53þ/� versus p53þ/þ mice. The overall difference was
small, but it was consistent with an increase in the incidence
of OTA-induced apoptosis in kidney OSOM and cortex of
p53-deficient gpt d mice compared to their p53-proficient
counterparts exposed to 1- or 5-mg OTA/kg BW by gavage for
4 weeks (Hibi et al. 2013b). Global gene expression analyses of
the kidney outer medulla of gpt d rats exposed to OTA demon-
strated that there were changes in the expression of genes reg-
ulating p53-dependent and p53-independent apoptosis (Hibi
et al. 2013a, 2013b). This study indicates that OTA-induced
apoptosis is likely to be mediated in part by 1 or more p53-
independent pathways. Furthermore, since p53 activates both
pro- and antiapoptotic genes (Roos and Kaina 2013), reduced
expression of p53-dependent antiapoptotic genes associated
with DNA repair may also contribute to the higher incidence
of apoptotic cells in kidneys of p53-deficient mice exposed
to OTA.
TABLE 4.—Summary of severity and incidence of histologic lesions in kidneys from p53þ/þ and p53þ/� mice exposed to dietary OTA for 26
weeks.
Renal Lesion and Location
OTA Added to Diet (mg OTA/kg Diet, Weeks 3–26)
p53þ/þ p53þ/�
0 0.5 2 10 0 0.5 2 10
Apoptosis OSOMa 0.0 + 0.0b 0.1 + 0.3 0.7 + 0.5 2.4 + 0.7d 0.0 + 0.0 0.0 + 0.0 0.3 + 0.7 2.5 + 0.5d
0/10b 1/10 6/9c 9/9c 0/10 0/10 2/10 10/10
MR 0.0 + 0.0 0.0 + 0.0 1.3 + 0.7d 2.7 + 0.5d 0.0 + 0.0 0.0 + 0.0 0.7 + 0.8 2.8 + 0.4d
0/10 0/10 8/9 9/9 0/10 0/10 5/10 10/10
CL 0.0 + 0.0 0.0 + 0.0 0.8 + 0.8 2.0 + 0.0d 0.0 + 0.0 0.0 + 0.0 2.0 + 0.5d 2.3 + 0.5d
0/10 0/10 5/9 9/9 0/10 0/10 10/10 10/10
Karyomegaly OSOM 0.0 + 0.0 0.0 + 0.0 0.0 + 0.0 2.4 + 0.9d 0.0 + 0.0 0.0 + 0.0 0.4 + 0.5 2.7 + 0.8d
0/10 0/10 0/9 9/9 0/10 0/10 4/10 10/10
MR 0.0 + 0.0 0.0 + 0.0 1.4 + 0.7 3.4 + 0.5d 0.0 + 0.0 0.0 + 0.0 1.1 + 0.7 3.0 + 0.7d
0/10 0/10 8/9 9/9 0/10 0/10 8/10 10/10
CL 0.0 + 0.0 0.0 + 0.0 1.4 + 0.7d 2.0 + 0.5d 0.0 + 0.0 0.0 + 0.0 1.5 + 1.0d 2.3 + 0.5d
0/10 0/10 8/9 9/9 0/10 0/10 8/10 10/10
Tubular degeneration OSOM 0.0 + 0.0 0.1 + 0.3 0.2 + 0.7 3.0 + 0.0d 0.0 + 0.0 0.1 + 0.3 0.0 + 0.0 3.0 + 0.0d
0/10 1/10 1/9 9/9 0/10 1/10 0/10 10/10
MR 0.0 + 0.0 0.0 + 0.0 1.3 + 1.0 3.0 + 0.0d 0.0 + 0.0 0.0 + 0.0 0.0 + 0.0 3.0 + 0.0d
0/10 0/10 6/9 9/9 0/10 0/10 0/10 10/10
CL 0.0 + 0.0 0.1 + 0.3 1.0 + 0.9 3.0 + 0.0d 0.0 + 0.0 0.0 + 0.0 1.4 + 0.7d 2.9 + 0.6d
0/10 1/10 6/9 9/9 0/10 0/10 9/10 10/10
Anisokaryosis OSOM 0.0 + 0.0 0.6 + 0.5 1.0 + 0.5 3.7 + 0.5d 0.0 + 0.0 0.2 + 0.4 1.3 + 0.7d 4.0 + 0.0d
0/10 4/10 8/9 9/9 0/10 2/10 9/10 10/10
MR 0.0 + 0.0 0.1 + 0.3 2.0 + 0.0d 3.8 + 0.4d 0.0 + 0.0 0.2 + 0.4 2.0 + 0.8d 3.7 + 0.5d
0/10 1/10 9/9 9/9 0/10 1/10 9/10 10/10
CL 0.0 + 0.0 0.2 + 0.4 1.3 + 1.0 2.1 + 0.9d 0.0 + 0.0 0.2 + 0.4 2.1 + 0.9d 3.0 + 0.5d
0/10 2/10 6/9 8/9 0/10 2/10 9/10 10/10
aOSOM ¼ outer stripe of outer medulla; MR ¼ medullary rays; CL ¼ cortical labyrinth. bSeverity data are expressed as mean + SD for lesion severity scores from 0 to 5, where
increasing scores are indicative of increasing lesion severity. Incidence data are expressed as # affected animals/total number animals per group. cHydronephrosis was observed in one
kidney in the medium-dose group and no further morphological changes were assessed; one kidney in the high-dose group was compromised at collection and could not be assessed.dLesion severity was significantly different from corresponding controls using analysis of variance (ANOVA) on ranks followed by post hoc pairwise comparisons using the Dunn’s or
Tukey test (p � .05).
Vol. XX, No. X, 2015 OCHRATOXIN A EFFECTS ON P53þ/� MICE 9
OTA stimulates and disrupts cell division in the kidney. A
dose-dependent increase in PCNA-positive cells, indicative
of proliferation, was observed in proximal tubules of p53þ/þand p53þ/� mice and was consistent with similar increases
in PCNA-positive proximal tubule cells in rats exposed to OTA
by gavage (Mally et al. 2005; Taniai et al. 2014). The presence
of cells with an abnormally enlarged nucleus, or karyomegaly,
in the renal proximal tubule is a distinguishing lesion associ-
ated with OTA exposure (Boorman et al. 1992). Although kar-
yomegaly can be induced by renal carcinogens, it is not
considered a preneoplastic lesion because there is no evidence
that proliferative foci stem directly from these cells (Hard et al.
1999). OTA and other karyomegaly-inducing carcinogens,
which also stimulated cellular proliferation, increased the
expression of gH2AX, a phosphorylated variant of the histone
H2AX involved in DNA double strand break (DSB) repair, in
the kidney OSOM of rats exposed to 210-mg OTA/kg bw/d
by gavage for 28 days (Taniai et al. 2012a). Phosphorylated
Chk2 and nuclear cdc2, both part of the G2/M DNA damage
checkpoint pathway, were also elevated suggesting that DNA
damage is associated with exposure to karyomegaly-inducing
carcinogens, triggering homeostatic repair responses that pre-
vent cells with DNA damage from entering mitosis. Multiple
epigenetic effects resulting in cell cycle perturbation have been
linked experimentally to OTA toxicity and carcinogenicity,
including aberrant ubiquitin D activation leading to disrupted
cell cycle regulation, inhibition of histone aceytltransferases
leading to mitotic disruption, and cytoskeletal perturbations
leading to aberrant cell division (Taniai et al. 2012b; Czakai
et al. 2011; Rached et al. 2006). One or more of these events
leading to mitotic disruption in renal proximal tubule cells
could manifest as OTA-induced karyomegaly. The hypothesis
that OTA-induced aberrant mitosis is a trigger for proliferative
changes in renal proximal tubules is plausible (Rached et al.
2007; Mally 2012), but the key event has yet to be conclusively
confirmed and the available evidence does not rule out multiple
cellular targets for OTA. Marin-Kuan et al. (2008) proposed
that OTA carcinogenicity stems from multiple epigenetic
mechanisms, including cell- and tissue-level responses to
OTA-meditated apoptosis, and tissue regeneration and prolif-
eration resulting from cytotoxicity due to oxidative stress and
protein synthesis inhibition. This hypothesis accommodates the
spectrum of cellular changes observed in kidneys from OTA-
exposed p53þ/þ and p53þ/� mice that ranged from necrosis
FIGURE 5.—Photomicrographs of kidney tissues from control mice and
mice exposed to ochratoxin A (OTA) in diet: (A) kidney cortex from a
p53þ/� control mouse; (B) kidney cortex from a p53þ/� mouse
exposed to 10-mg OTA/kg diet. In (B), the large black arrowheads
indicate proximal convoluted tubular epithelial cell with karyome-
galy, the white arrowheads indicate apoptotic bodies, and the arrows
indicate damaged tubules containing vacuolated epithelial cells.
Hematoxylin and eosin stain; scale bars 50 mm.
FIGURE 6.—Photomicrograph of a lung section from a p53þ/� control
mouse; hematoxylin and eosin stain. A large needle-shaped crystal is
evident in the bronchiole (black arrowhead); in the adjacent alveoli, a
light mixed leukocytic infiltration composed of macrophages with
acidophilic cytoplasm and a few neutrophils is evident. Hematoxylin
and eosin stain; scale bar 100 mm.
10 BONDY ET AL. TOXICOLOGIC PATHOLOGY
TABLE 5.—Immunohistochemical assessment of kidneys from p53þ/þ and p53þ/� mice exposed to dietary OTA for 26 weeks.
Endpointa
OTA Added to Diet (mg OTA/kg diet, Weeks 3–26)
p53þ/þ p53þ/�
0 0.5 2 10 0 0.5 2 10
# PCNA positive cells 385.6 + 55.3 441.5 + 122.7 519.0 + 31.3 738.8 + 93.4b 389.9 + 41.7 478.1 + 48.6 455.0 + 105.6 799.2 + 83.7b
# Apoptotic cells 453.3 + 40.7 453.3 + 75.8 551.0 + 27.4 729.6 + 55.6b 471.1 + 47.3 499.1 + 22.7c 550.9 + 24.7 817.2 + 83.4b,c
Clusterin expression 18.5 + 6.7 29.0 + 16.1 33.3 + 15.4 47.5 + 12.7b 21.6 + 8.1 34.5 + 13.8 40.5 + 16.9b 50.0 + 7.5b
Osteopontin expression 27.0 + 9.5 42.5 + 17.5 53.9 + 12.4 75.5 + 6.0b 30.5 + 10.9 51.0 + 14.9 59.0 + 13.7b 81.0 + 8.4b
aData are expressed as meanþ SD of # proliferating cell nuclear antigen (PCNA) positive/mm2 cells or # apoptotic cells/mm2 in proximal tubules of 1 kidney section/mouse. Clusterin
and osteopontin expression data are expressed as mean þ SD of semiquantitative percentage positivity scores for proximal tubule staining on 1 kidney section/mouse as described in the
Methods and Materials. For each endpoint, 1 kidney section was assessed for a total n ¼ 9 or 10 mice/dose/strain (as in Table 4). bData are significantly different from corresponding
controls using analysis of variance (ANOVA) on Ranks followed by post hoc pairwise comparisons using the Dunn’s test (p � .05). cData are significantly different from corresponding
p53þ/þ mice using 2-way ANOVA on Ranks followed by post hoc pairwise comparisons using the Dunn’s test (p � .05).
FIGURE 7.—Clusterin (CLU) and osteopontin (OPN) expression in the outer stripe of the outer medulla of kidneys from p53þ/þ mice: (A)
CLU, control; (B) CLU, 10-mg ochratoxin A (OTA)/kg diet; (C) OPN, control; (D) OPN, 10-mg OTA/kg diet. CLU and OPN positivity are
visible as dark reddish-brown staining, more prominent in kidney sections from the 10-mg OTA/kg dose group. Scale bars 100 mm.
Vol. XX, No. X, 2015 OCHRATOXIN A EFFECTS ON P53þ/� MICE 11
and apoptosis to proliferation and changes such as karyome-
galy, anisokaryosis, and hyperchromatic nuclei in renal epithe-
lial cells.
Based on experimental evidence of OTA carcinogenicity in
rats, mice, and poultry (Bendele et al. 1985; NTP 1989; Stoev
2010), DNA damage is a likely outcome of OTA exposure. In
confirmation, in vivo mutagenesis assays using gpt d rats
detected large deletion mutations in the outer medulla of the
kidney after 4 weeks of exposure to 5-mg/kg OTA by gavage
(Hibi et al. 2011). Positive comet assays and increased phos-
phorylation of histone variant H2AX were indicative of DNA
DSBs at the target site and increased expression of genes linked
to DNA repair by homologous recombination (HR) suggested
that large deletion mutations may arise during repair by HR
of OTA-induced DSBs (Kuroda et al. 2014). However, the
underlying mechanism of OTA-induced DSBs has yet to be
determined. Nuclear 8-hydroxy-20-deoxyguanosine (8-OHdG)
levels were not altered in the cortex or outer medulla of gpt drats exposed to OTA, suggesting that oxidative DNA damage
was not the primary cause of deletion mutations at the target
site in this model (Hibi et al. 2011), but other epigenetic path-
ways leading to OTA-induced genotoxicity cannot be ruled out
(Mally and Dekant 2009; Trosko and Ruch 1998).
Changes in CLU and OPN expression in kidneys from
p53þ/þ and p53þ/� mice were similar to those seen in kid-
neys from OTA-exposed rats (Rached et al. 2008). Dose-
dependent increases in CLU and OPN positivity in proximal
and distal tubules due to OTA exposure in mice were consistent
with their identification as presumptive biomarkers of both
proximal and distal tubule injury (Hoffmann et al., 2010).
Although CLU and OPN have been used as renal injury mar-
kers, both are widely distributed in tissues. The secretory het-
erodimeric glycoprotein CLU has been reported to be
involved in regulating multiple cellular responses that may
occur in a mutually exclusive and opposing manner, for exam-
ple, apoptotic cell death, cell cycle regulation, DNA repair, cell
adhesion, tissue remodeling, lipid transportation, membrane
recycling, and immune system regulation (Jones and Jomary
2002; Shannan et al. 2006). OPN, a secretory glycosylated
phosphoprotein, is an antiapoptotic factor associated with reg-
ulation of bone remodeling, chemotaxis, and immune
responses, as well as cellular proliferation and regeneration
after renal injury (Xie et al. 2001). Consequently, increased
renal CLU and OPN expression in OTA-exposed mice are con-
sistent with an increased incidence of proliferating cells, apop-
totic cells, necrosis, and other lesions indicative of cell cycle
disruption.
There were no significant changes in peripheral and splenic
WBC numbers, including granulocyte differentials and lym-
phocyte subsets, in p53þ/þ and p53þ/� mice chronically
exposed to OTA. Similarly, there were no significant changes
in peripheral WBC numbers in rats chronically exposed to
OTA in diet (NTP 1989). Mild splenomegaly in all high-dose
p53þ/þ and p53þ/� mice was most likely a nonspecific
response to tissue damage in target organs such as the kidney.
Cellular proliferation was significantly depressed in ex vivo
splenocyte cultures indicating functional compromise in lym-
phocytes from OTA-exposed mice, which was generally in
accordance with the well-established immunosuppressive
effects of OTA (Bondy and Pestka 2000).
The lung lesions observed in all p53þ/� and p53þ/þ mice
were unexpected but not considered to be treatment related.
ECP is a sporadic, idiopathic disease that occurs in certain
strains of laboratory mice, including the C57BL/6 and 129Sv
strains used to generate this p53þ/� knockout and the reconsti-
tuted p53þ/þ mouse (French, Storer, and Donehower 2001b;
Hoenerhoff, Starost, and Ward 2006). To our knowledge, this
is the first report of ECP in this mouse model. The disease was
considered mild, but there was apparent exacerbation with
OTA treatment resulting in a slight increase in the severity of
ECP in high-dose mice. Since ECP has been associated with
mutations that result in immunodeficiency or that target the
immune system (Guo, Johnson, and Schuh 2000), it is possible
that OTA-induced immunosuppression contributed to
increased ECP severity. The pulmonary smooth muscle hyper-
plasia that was also observed in all mice is unexplained at this
time but was not considered to be treatment related and was not
increased in severity with OTA exposure.
OTA is nephrotoxic to laboratory and domestic animals and,
irrespective of its MOA, is considered a potential human health
hazard. The lowest observed effect level (LOEL) for renal toxi-
city in the pig, which is highly sensitive to OTA-induced
nephrotoxicity, was 8-mg/kg BW/day for minimal renal toxicity
(JECFA 2008; Krogh et al. 1974). The LOEL for renal proxi-
mal tubule karyomegaly in male rats exposed to OTA by
gavage for 5 d/wk for 90 d was 62.5 mg/kg BW/d (NTP
1989). In 2-year carcinogenesis studies the LOEL for kidney
tumors was 4,400 mg/kg BW/d in male B6C3F1 mice exposed
to OTA in diet, and 70 mg/kg BW/d in male rats exposed to
OTA by gavage for 5 d/wk (Bendele et al. 1985; JECFA
2008; NTP 1989). In comparison, the lowest dose group in
which renal changes were observed in p53þ/� and p53þ/þmice was 2-mg OTA/kg diet, corresponding to a LOEL of
200-mg OTA/kg BW/day based on feed consumption. This is
lower than the LOEL for kidney tumors in B6C3F1 mice,
although the wide dose separation between the 1 ppm and 40
ppm dietary OTA levels in the 2-year mouse study complicates
direct comparison with the present study. Taken together, these
comparisons support the general conclusion that mice are less
sensitive than rats and pigs to OTA-induced nephrotoxicity and
less sensitive than rats to OTA-induced renal carcinogenesis.
Species sensitivity was arguably a more critical influence on
responses to OTA than p53 heterozygosity.
In conclusion, renal changes due to ochratoxicosis in
p53þ/þ and p53þ/�mice were consistent with those observed
in B6C3F1 mice and in other species. Heterozygosity for the
p53 gene had a limited influence on murine responses to OTA.
The results of this study were interpreted to be suggestive of
primarily epigenetic MOAs for OTA carcinogenesis, based
on validation of the p53þ/� N5 mouse for use in short-term
carcinogenesis bioassays which has shown that this model is
susceptible to tumor induction by genotoxic and not
12 BONDY ET AL. TOXICOLOGIC PATHOLOGY
nongenotoxic carcinogens (Pritchard et al. 2003; Tennant,
Spalding, and French 1996).
ACKNOWLEDGMENTS
The authors would like to thank Jennifer Eastwood, Mark
Feeley, Gary Lombaert, and Tim Schrader for valuable discus-
sions and article review, and the staff of the Health Canada
animal care facility for their assistance throughout the study.
AUTHOR CONTRIBUTION
Authors contributed to conception or design (GB, LC, IC,
DL, and RM); data acquisition, analysis, or interpretation
(GB, DC, SA, LC, CA, IC, RK, KK, DL, and RM); drafting the
manuscript (GB); critically revising the manuscript (DC, SA,
LC, CA, DL, and RM); and gave final approval (RM). All
authors gave final approval, all authors agreed to be accounta-
ble for all aspects of work in ensuring that questions relating to
the accuracy or integrity of any part of the work are appropri-
ately investigated and resolved.
REFERENCES
Armed Forces Institute of Pathology. (2008). Accession No. 3095070. US
Department of Defense, Washington, DC.
Barlow, S., Renwick, A. G., Kleiner, J., Bridges, J. W., Busk, L., Dybing, E.,
Edler, L., et al. (2006). Risk assessment of substances that are both geno-
toxic and carcinogenic. Report of an International Conference organized
by EFSA and WHO with support of ILSI Europe. Food Chem Tox 44,
1636–50.
Battacone, G., Nudda, A., and Pulina, G. (2010). Effects of ochratoxin A on
livestock production. Toxins (Basel) 2, 1796–824.
Bendele, A. M., Carlton, W. W., Krogh, P., and Lillehoj, E. B. (1985). Ochra-
toxin A carcinogenesis in the (C57BL/6J x C3H)F1 mouse. J Nat Canc Inst
75, 733–42.
Bondy, G., Mehta, R., Caldwell, D., Coady, L., Armstrong, C., Savard, M.,
Miller, J. D., Chomyshyn, E., Bronson, R., Zitomer, N., and Riley, R. T.
(2012). Effects of long term exposure to the mycotoxin fumonisin B1 in
p53 heterozygous and p53 homozygous transgenic mice. Food Chem Tox
50, 3604–13.
Bondy, G. S., and Pestka, J. J. (2000). Immunomodulation by fungal toxins. J
Tox Env Health Pt B 3, 109–43.
Boorman, G. A., McDonald, M. R., Imoto, S., and Persing, R. (1992). Renal
lesions induced by ochratoxin A exposure in the F344 rat. Tox Path 20,
236–45.
Bui-Klimke, T., and Wu, F. (2014). Ochratoxin A and human health risk: A
review of the evidence. Crit. Rev. Food Sci Nutr, accessed January 7,
2015, http://dx.doi.org/10.1080/10408398.2012.724480.
Czakai, K., Muller, K., Mosesso, P., Pepe, G., Schulze, M., Gohla, A., Patnaik,
D., Dekant, W., Higgins, J. M. G., and Mally, A. (2011). Perturbation of
mitosis through inhibition of histone acetyltransferases: The key to ochra-
toxin A toxicity and carcinogenicity? Tox Sci 122, 317–29.
Delatour, T., Mally, A., Richoz, J., Ozden, S., Dekant, W., Ihmels, H., Otto, D.,
Gasparutto, D., Marin-Kuan, M., Schilter, B., and Cavin, C. (2008).
Absence of 2’-deoxyguanosine-carbon 8-bound ochratoxin A adduct in rat
kidney DNA monitored by isotope dilution LC-MS/MS. Mol Nutr Food
Res 52, 472–82.
Donehower, L. A., Harvey, M., Slagle, B. L., McArthur, M. J., Montgomery,
C. A. Jr., Butel, J. S., and Bradley, A. (1992). Mice deficient for p53 are
developmentally normal but susceptible to spontaneous tumours. Nature
356, 215–21.
Duarte, S. C., Pena, A., and Lino, C. M. (2010). A review on ochratoxin A
occurrence and effects of processing of cereal and cereal-derived food
products. Food Micro 27, 187–98.
Dunnick, J. K., Hardisty, J. F., Herbert, R. A., Seeley, J. C., Furedi-Machacek,
E. M., Foley, J. F., Lacks, G. D., Stasiewicz, S., and French, J. E. (1997).
Phenolphthalein induces thymic lymphomas accompanied by loss of the
p53 wild type allele in heterozygous p53-deficient (+) mice. Tox Path
25, 533–40.
European Food Safety Authority. (2005). Opinion of the Scientific Committee
on a request from EFSA related to a harmonized approach for risk assess-
ment of substances which are both genotoxic and carcinogenic. EFSA J
282, 1–31.
Floyd, E., Mann, P., Long, G., and Ochoa, R. (2002). The Trp53 hemizygous
mouse in pharmaceutical development: Points to consider for pathologists.
Tox Path 30, 147–56.
Foley, G. L. (2001). Overview of male reproductive pathology. Tox Path 29,
49–63.
Frazier, K. S., Seeley, J. C., Hard, G. C., Betton, G., Burnett, R., Nakatsuji, S.,
Nishikawa, A., Durchfield-Meyer, B., and Bube, A. (2012). Proliferative
and nonproliferative lesions of the rat and mouse urinary system. Tox Path
40, 14S–86S.
French, J. E., Lacks, G. D., Trempus, C., Dunnick, J. K., Foley, J., Mahler, J.,
Tice, R. R., and Tennant, R. (2001a). Loss of heterozygosity frequency at
the Trp53 locus in p53-deficient (þ/-) mouse tumors is carcinogen- and tis-
sue-dependent. Carcinogenesis 21, 99–106.
French, J., Storer, R. D., and Donehower, L. A. (2001b). The nature of the het-
erozygous Trp53 knockout model for identification of mutagenic carcino-
gens. Tox Path 29, 24–29.
Grollman, A. P., Shibutani, S., Moriya, M., Miller, F., Wu, L., Moll, U.,
Suzuki, N., et al. (2007). Aristolochic acid and the etiology of endemic
(Balkan) nephropathy. Proc Nat Acad Sci USA 104, 12129–34.
Guo, L., Johnson, R. S., and Schuh, J. C. L. (2000). Biochemical characteriza-
tion of endogenously formed eosinophilic crystals in the lungs of mice. J
Biol Chem 275, 8032–37.
Hard, G. C., Alden, C. L., Bruner, R. H., Frith, C. H., Lewis, R. M., Owen, R.
A., Krieg, K., and Durchfeld-Meyer, B. (1999). Non-proliferative lesions of
the kidney and lower urinary tract in rats. In Guides for Toxicologic Pathol-
ogy, pp. 1–32. STP/ARP/AFIP, Washington, DC.
Harris, S. L., and Levine, A. J. (2005). The p53 pathway: Positive and negative
feedback loops. Oncogene 24, 2899–908.
Hibi, D., Suzuki, Y., Ishii, Y., Jin, M., Watanabe, M., Sugita-Konishi, Y.,
Yanai, T., Nohmi, T., Nishikawa, A., and Umemura, T. (2011). Site-
specific in vivo mutagenicity in the kidney of gpt delta rats given a carci-
nogenic dose of ochratoxin A. Tox Sci 122, 406–14.
Hibi, D., Kijima, A., Kuroda, K., Suzuki, Y., Ishii, Y., Jin, M., Nakajima, M.,
Sugita-Konishi, Y., Yanai, T., Nohmi, T., Nishikawa, A., and Umemura, T.
(2013a). Molecular mechanisms underlying ochratoxin A-induced geno-
toxicity: Global gene expression analysis suggests induction of DNA
double-strand breaks and cell cycle progression. J Tox Sci 38, 57–69.
Hibi, D., Kijima, A., Suzuki, Y., Ishii, Y., Jin, M., Sugita-Konishi, Y., Yanai, T.,
Nishikawa, A., and Umemura, T. (2013b). Effects of p53 knockout on ochra-
toxin A-induced genotoxicity in p53-deficient gpt delta mice. Toxicology
304, 92–99.
Hoenerhoff, M. J., Starost, M. F., and Ward, J. M. (2006). Eosinophilic crystal-
line pneumonia as a major cause of death in 129S4/SvJae mice. Vet Path
43, 682–8.
Hoffman, W. P., Ness, D. K., and van Lier, R. B. L. (2002). Analysis of rodent
growth data in toxicology studies. Tox Sci 66, 313–9.
Hoffmann, D., Fuchs, T. C., Henzler, T., Matheis, K. A., Herget, T., Dekant,
W., Hewitt, P., and Mally, A. (2010). Evaluation of a urinary kidney bio-
marker panel in rat models of acute and subchronic nephrotoxicity. Toxi-
cology 277, 49–58.
International Agency for Research on Cancer. (1993). Some Naturally Occur-
ring Substances: Food Items and Constituents, Heterocyclic Aromatic
Amines, and Mycotoxins. IARC Monographs on the Evaluation of Carci-
nogenic Risk of Chemicals to Humans, Vol. 56. International Agency for
Research on Cancer, Lyon, France. Accessed January 7, 2015, http://mono-
graphs.iarc.fr/ENG/Monographs/vol56/mono56.pdf.
International Collaborative Immunotoxicity Study. (1998). Report of valida-
tion study of assessment of direct immunotoxicity in the rat. The ICICIS
Vol. XX, No. X, 2015 OCHRATOXIN A EFFECTS ON P53þ/� MICE 13
Group Investigators. International Collaborative Immunotoxicity Study.
Toxicology 125, 183–201.
Joint FAO/WHO Expert Committee on Food Additives. (2008). Safety evalua-
tion of certain food additives and contaminants: Ochratoxin A (addendum).
In WHO Food Additives Series: 59, pp. 357–429. International Programme
on Chemical Safety, World Health Organization, Geneva.
Jennings, P., Welland, C., Limonciel, A., Bloch, K. M., Radford, R., Aschauer,
L., McMorrow, T., Wilmes, A., et al. (2012). Transcriptomic alterations
induced by ochratoxin A in rat and human renal proximal tubular in vitro
models and comparison to a rat in vivo model. Arch Tox 86, 571–89.
Jha, V., Garcia-Garcia, G., Iseki, K., Li, Z., Naicker, S., Plattner, B., Saran, R.,
Wang, A. Y. M., and Wang, C. W. (2013). Chronic kidney disease: Global
dimension and perspectives Lancet 382, 260–72.
Jones, S. E., and Jomary, C. (2002). Molecules in focus: Clusterin. Int J Bio-
chem Cell Biol 34, 427–31.
Kanisawa, M., and Suzuki, S. (1978). Induction of renal and hepatic tumors in
mice by ochratoxin A, a mycotoxin. Gann 69, 599–600.
Krogh, P., Axelson, N. H., Elling, F., Gyrd-Hansen, N., Hald, B., Hyldgaard-
Jensen, J., Larsen, A. E., Madsen, A., et al. (1974). Experimental porcine
nephropathy. Acta Path Micro Scand A Suppl 246, 1–21.
Krogh, P., Elling, F., Friis, C., Hald, B., Larsen, A. E., Lillehøj, E. B., Madsen,
A., Mortensen, P., Rasmussen, F., and Ravnskov, U. (1979). Porcine
nephropathy induced by long-term ingestion of ochratoxin A. Vet Path
16, 466–75.
Kuiper-Goodman, T., Hilts, C., Billiard, S. M., Kiparissis, Y., Richard, I. D. K.,
and Hayward, S. (2010). Health risk assessment of ochratoxin A for all age-
sex strata in a market economy. Food Addit Contam 27, 212–40.
Kuroda, K., Hibi, D., Ishii, Y., Takasu, S., Kijima, A., Matsushita, K., Masu-
mura, K., Watanabe, M., Sugita-Konishi, Y., Sakai, H., Yanai, T., Nohmi,
T., Ogawa, K., and Umemura, T. (2014). Ochratoxin A induces DNA
double-strand breaks and large deletion mutations in the carcinogenic tar-
get site of gpt delta rats. Mutagenesis 29, 27–36.
Lanning, L. L., Creasy, D. M., Chapin, R. E., Mann, P. C., Barlow, N. J.,
Regan, K. S., and Goodman, D. G. (2002). Recommended approaches for
the evaluation of testicular and epididymal toxicity. Tox Path 30, 507–20.
Lombaert, G. A., Pellaers, P., Roscoe, V., Mankotia, M., Neil, R., and Scott, P.
M. (2003). Mycotoxins in infant cereal foods from the Canadian retail mar-
ket. Food Addit Contam 20, 494–504.
Luna, L. G. (1968). Manual of histologic staining methods of Armed Forces
Institute of Pathology. 3rd ed, McGraw-Hill, Toronto, ON, Canada.
Mally, A. (2012). Ochratoxin A and mitotic disruption: Mode of action analysis
of renal tumor formation by ochratoxin A. Tox Sci 127, 315–30.
Mally, A., Decker, M., Bekteshi, M., and Dekant, W. (2006). Ochratoxin A
alters cell adhesion and gap junction intercellular communication in
MDCK cells. Toxicology 223, 15–25.
Mally, A., and Dekant, W. (2009). Mycotoxins and the kidney: Modes of action
for renal tumor formation by ochratoxin A in rodents. Mol Nutr Food Res
53, 467–78.
Mally, A., Volkel, W., Amberg, A., Kurz, M., Wanek, P., Eder, E., Hard, G.,
and Dekant, W. (2005). Functional, biochemical, and pathological effects
of repeated oral administration of ochratoxin A to rats. Chem Res Tox
18, 1242–52.
Mantle, P. G., Faucet-Marquis, V., Manderville, R. A., Squillaci, B., and Pfohl-
Leskowicz, A. (2010). Structures of covalent adducts between DNA and
ochratoxin A: A new factor in debate about genotoxicity and human risk
assessment. Chem Res Tox 23, 89–98.
Marin, S., Ramos, A. J., Cano-Sancho, G., and Sanchis, V. (2013). Mycotoxins:
Occurrence, toxicology, and exposure assessment. Food Chem Tox 60,
218–37.
Marin-Kuan, M., Cavin, C., Delatour, T., and Schilter, B. (2008). Ochratoxin A
carcinogenicity involves a complex network of epigenetic mechanisms.
Toxicon 52, 195–202.
Marin-Kuan, M., Ehrlich, V., Delatour, T., Cavin, C., and Schilter, B. (2011).
Evidence for a role of oxidative stress in the carcinogenicity of ochratoxin
A. J Tox, 2011: 645361, 1–15, doi:10.1155/2011/645361.
Marin-Kuan, M., Nestler, S., Verguet, C., Bezencon, C., Piguet, D., Mansour-
ian, R., Holzwarth, R., Grigorov, M., Delatour, T., Mantle, P., Cavin, C.,
and Schilter, B. (2006). A toxicogenomics approach to identify new plau-
sible epigenetic mechanisms of ochratoxin A carcinogenicity in rat. Tox Sci
89, 120–34.
McClellan, W. M., and Flanders, W. D. (2003). Risk factors for progressive
chronic kidney disease. J Am Soc Nephrol 14, S65–S70.
National Toxicology Program. (1989). Toxicology and carcinogenesis studies
of ochratoxin A (CAS No. 303-47-9) in F344/N rats (gavage studies). NTP
TR 358, NIH Publication No. 89-2813., US Department of Health and
Human Services, Research Triangle Park, NC.
National Toxicology Program. (2005a). Toxicity studies of acesulfame potas-
sium (CAS NO. 55589-62-3) in FVB/N-TgN(v-Ha-ras)Led (Tg.AC) hemi-
zygous mice and carcinogenicity studies of acesulfame potassium in B6.
129-Trp53tm1Brd(N5) haploinsufficient mice. NTP GMM 2, NIH Publica-
tion No. 06-4460, US Department of Health and Human Services, Research
Triangle Park, NC.
National Toxicology Program. (2005b). Toxicology studies of aspartame (CAS
NO. 22839-47-0) in genetically modified (FVB Tg.AC hemizygous) and
B6.129-Cdkn2atm1Rdp(N2) deficient mice and carcinogenicity studies of
aspartame in genetically modified [B6.129-Trp53tm1Brd(N5) haploinsuffi-
cient] mice. NTP GMM 1, NIH Publication No. 06-4459, US Department
of Health and Human Services, Research Triangle Park, NC.
Ominski, K. H., Marquardt, R. R., Sinha, R. N., and Abramson, D. (1994). Eco-
logical aspects of growth and mycotoxin production by storage fungi. In
Mycotoxins in Grain: Compounds Other Than Aflatoxin (J. D. Miller and
H. L. Trenholm, Eds.), pp. 287–312. Eagan Press, St. Paul, MN.
Pfohl-Leszkowicz, A. (2009). Ochratoxin A and aristolochic acid involvement
in nephropathies and associated urothelial tract tumours. Arh Hig Rada
Toksikol 60, 465–83.
Pritchard, J. B., French, J. E., Davis, B. J., and Haseman, J. K. (2003). The role
of transgenic mouse models in carcinogen identification. Env Health Per-
spect 111, 444–54.
Rached, E., Pfeiffer, E., Dekant, W., and Mally, A. (2006). Ochratoxin A:
Apoptosis and aberrant exit from mitosis due to perturbation of microtubule
dynamics. Tox Sci 92, 78–86.
Rached, E., Hard, G. C., Blumbach, K., Weber, K., Draheim, R., Lutz, W.K.,
Ozden, S., Steger, U., Dekant, W., and Mally, A. (2007). Ochratoxin A: 13-
week oral toxicity and cell proliferation in male F344/N rats. Tox Sci 97,
288–98.
Rached, E., Hoffman, D., Blumbach, K., Weber, K., Dekant, W., and Mally, A.
(2008). Evaluation of putative biomarkers of nephrotoxicity after exposure
to ochratoxin A in vivo and in vitro. Tox Sci 103, 371–81.
Roos, W. P., and Kaina, B. (2013). DNA damage-induced cell death: From spe-
cific DNA lesions to the DNA damage response and apoptosis. Canc Lett
332, 237–48.
Shannan, B., Seifert, M., Leskov, K., Willis, J., Boothman, D., Tilgen, W., and
Reichrath, J. (2006). Challenge and promise: roles for clusterin in patho-
genesis, progression and therapy of cancer. Cell Death Diff 13, 12–19.
Sharma, P., Manderville, R. A., and Wetmore, S. D. (2013). Modeling the
conformational preference of the carbon-bonded covalent adduct formed
upon exposure of 2’-deoxyguanosine to ochratoxin A. Chem Res Tox 26,
803–16.
Stefanovic, V., Polenakovic, M., and Toncheva, D. (2011). Urothelial carci-
noma associated with Balkan endemic nephropathy: A worldwide disease.
Path Biol (Paris) 59, 286–91.
Stoev, S. D. (2010). Studies on carcinogenic and toxic effects of ochratoxin A
in chicks. Toxins (Basel) 2, 649–64.
Taniai, E., Hayashi, H., Yafune, A., Watanabe, M., Akane, H., Suzuki, K., Mit-
sumori, K., and Shibutani, M. (2012a). Cellular distribution of cell cycle-
related molecules in the renal tubules of rats treated with renal carcinogens
for 28 days: relationship between cell cycle aberration and carcinogenesis.
Arch Tox 86, 1453–64.
Taniai, E., Yafune, A., Hayashi, H., Itahashi, M., Hara-Kudo, Y., Suzuki, K.,
Mitsumori, K., and Shibutani, M. (2012b). Aberrant activation of ubiquitin
D at G2 phase and apoptosis by carcinogens that evoke cell proliferation
after 28-day administration in rats. J Tox Sci 37, 1093–111.
Taniai, E., Yafune, A., Nakajima, M., Hayashi, S. M., Nakane, F., Itahashi, M.,
and Shibutani, M. (2014). Ochratoxin A induces karyomegaly and cell
14 BONDY ET AL. TOXICOLOGIC PATHOLOGY
cycle aberrations in renal tubular cells without relation to induction of
oxidative stress responses in rats. Tox Let 224, 64–72.
Tennant, R. W., Spalding, J., and French, J. E. (1996). Evaluation of transgenic
mouse bioassays for identifying carcinogens and noncarcinogens. Mut Res
365, 119–27.
Trosko, J. E., and Ruch, R. J. (1998). Cell-cell communication in carcinogen-
esis. Front Biosci 3, 208–36.
Tryphonas, H., Cooke, G., Caldwell, D., Bondy, G., Parenteau, M., Hayward,
S., and Pulido, O. (2004). Oral (gavage), in utero and post-natal exposure of
Sprague-Dawley rats to low doses of tributyltin chloride: Part II: effects on
the immune system. Food Chem Tox 42, 221–35.
van der Merwe, K. J., Steyn, P. S., Fourie, L., Scott, De B., and Theron, J. J.
(1965). Ochratoxin A, a toxic metabolite produced by Aspergillus ochra-
ceus Wilh. Nature 205, 1112–3.
Varga, J., Rigo, K., Teren, J., and Mesterhazy, A. (2001). Recent advances in
ochratoxin research. I. Production, detection and occurrence of ochratox-
ins. Cereal Res Comm 29, 85–92.
Wu, F., and Wang, T. (2013). Risk assessment of upper tract urothelial carcinoma
related to aristolochic acid. Canc Epidemiol Biomarkers Prev 22, 812–20.
Xie, Y., Sakatsume, M., Nishi, S., Narita, I., Arakawa, M., and Gejyo, F.
(2001). Expression, roles, receptors, and regulation of osteopontin in the
kidney. Kid Int 60, 1645–57.
For reprints and permissions queries, please visit SAGE’s Web site at http://www.sagepub.com/journalsPermissions.nav.
Vol. XX, No. X, 2015 OCHRATOXIN A EFFECTS ON P53þ/� MICE 15