Printer Friendly

Cross-talk in the female rat mammary gland: influence of aryl hydrocarbon receptor on estrogen receptor signaling.


To evaluate the influence of endocrine-disrupting natural compounds or selective estrogen receptor modulators, it is crucial to understand the underlying mechanisms. This study was designed to investigate the impact of ligand-activated aryl hydrocarbon receptor (AHR) on ligand-activated estrogen receptor (ER) signaling pathways in the rodent mammary gland.

The AHR is a ligand-dependent transcription factor that belongs to the basic helixloop-helix/Per-Arnt-Sim (bHLH/PAS) family (Hankinson 1995; Matsumura and Vogel 2006; Mimura and Fujii-Kuriyama 2003; Poellinger 2000). The best-characterized ligands for the AHR are planar hydrophobic molecules, including many environmental contaminants such as halogenated aromatic hydrocarbons (HAHs) and polycyclic aromatic hydrocarbons (PAHs) (reviewed by Denison et al. 2002). After ligand binding, AHR translocates to the nucleus, dimerizes with its partner protein, aryl hydrocarbon receptor nuclear translocator (ARNT), and the AHR/ARNT-heterodimer binds to xenobiotic response elements (XREs), inducing gene expression for drug-metabolizing enzymes such as CYP1A1 and CYP1B1 (Beischlag et al. 2008; Larsen et al. 1998; Whitlock et al. 1996). In addition to its major role in xenobiotic metabolism, the AHR is involved in the regulation of cell proliferation, apoptosis, adipose differentiation, tumor suppressor functions, immune cell differentiation, and reproductive function (Hernandez-Ochoa et al. 2009; Kerkvliet 2002; Puga et al. 2009). The physiological consequences of these actions on individual tissues have not yet been fully elucidated. In the mammary gland, the AHR is dispensable for development (Le Provost et al. 2002), but this receptor appears to be an important factor in the regulation of proliferation because in AHR-null mice, the number of terminal end buds (TEBs) is reduced by 50% during estrous-stimulated growth (Hushka et al. 1998). These AHR-mediated responses in the mammary gland are most likely due to cross-talk between AHR and steroid receptors, including ER[alpha], ER[beta], and androgen receptor (AR), as has been reported for cell lines and mouse uterus (Beischlag and Perdew 2005; Matthews et al. 2005; Ohtake et al. 2003, 2007, 2008). How ligandactivated AHR influences ER signaling on a molecular level remains unclear. Several different mechanisms have been proposed, including direct binding to ERs, competition between the AHR/ARNT complex and the ER for common cofactors (p300, p160, CBP), induction of CYPs by activated AHR leading to enhanced E2 metabolism, and proteasomal degradation of the ER triggered by liganded AHR (for an overview, see Shanle and Xu 2011; Swedenborg and Pongratz 2010).

PAHs are widespread AHR ligands that mainly form in the process of incomplete combustion and are therefore abundant constituents of exhaust fumes from cars and factories as well as of cigarette smoke. Because the synthetic PAH 3-methylcholanthrene (3-MC) has a carcinogenic potential that is higher than that of most other PAHs such as benzo[a]pyrene, it is frequently employed to induce tumor formation in mice (Chen et al. 2015; Rymaszewski et al. 2014). Furthermore, 3-MC is frequently used in studies investigating AHR signaling because it is known to be a strong activator of AHR (Riddick et al. 1994). In addition, 3-MC is readily metabolized, further decreasing its effectiveness regarding the activation of AHR in vivo, whereas other AHR ligands such as 2,3,7,8-tetrachlorodibenzo-p-dioxin (TCDD) are extremely persistent (Riddick et al. 1994). This characteristic makes 3-MC a suitable model to study effects of PAHs on ER signaling. In this paper, we describe the in vivo effects of E2, 3-MC, and E2 + 3-MC on transcriptional and translational regulation of mRNA and protein levels to develop a mechanistic understanding of the interactions between AHR- and ER-mediated signaling pathways in the rat mammary gland in a physiol ogical context. We have used a transcriptome-based approach to characterize ER- and AHR-regulated genes and the overall expression change triggered by their respective receptors. Additionally, we treated rats with the potent phytoestrogen 8-prenylnaringenin (8-PN) (Milligan et al. 1999; Zierau et al. 2008) either alone or in co-treatment with 3-MC.


Substances. 17P-Estradiol (E2) and 3-methylcholanthrene (3-MC) were purchased from Sigma-Aldrich. 8-Prenylnaringenin (8-PN) was synthesized from naringenin as described previously (Gester et al. 2001). The purity of the compound was assessed to be > 99% by gas chromatography and high-performance liquid chromatography (HPLC). 8-PN was used as a racemic mixture.

Animals. Young adult female Lewis rats (200 g) were maintained under controlled conditions of temperature (20 [+ or -] 1[degrees]C, relative humidity 50-80%) and illumination (12 hr light, 12 hr dark). Animals were housed in open cages (Tecniplast) with four to six animals per cage. A mixture of Lignocell wood chips and Rehofix corncob granules (JRS Rettenmaier & Sohne) was used for bedding. All rats had free access to standard phytoestrogen-free rat diet (Teklad Global Diet) and water. Animals used in this study were treated humanely and with regard for the alleviation of suffering. The experimental design complied with the ARRIVE guidelines published by the National Centre for the Replacement, Refinement and Reduction of Animals in Research ( All procedures were approved by and carried out according to the institutional and state Animal Care and Use Committee guidelines mandated by the German federal law for animal welfare.

Three-day in vivo assay. Approximately 10-week-old rats were bilaterally ovariectomized (ovx). Fourteen days after ovx, rats were treated subcutaneously with the test compounds (E2, 3-MC, E2 + 3-MC, 8-PN, and 8-PN + 3-MC) in the same room in which the animals were housed. The animals were treated 2 hr after the start of the light period of the day; three treatments were administered at intervals of 24 hr. E2 was administered at 4 [micro]g/kg body weight (BW)/ day, and 3-MC and 8-PN were administered at 15 mg/kg BW/day. The combination doses for E2 + 3-MC were 4 [micro]g/kg BW + 15 mg/kg BW, respectively, and the doses for 8-PN + 3-MC were 15 mg/kg BW + 15 mg/kg BW, respectively. The substances were dissolved in a dimethyl sulfoxide (DMSO)/castor oil mixture that also served as the negative control (hereafter referred to as vehicle). The animals were randomly selected for treatment and vehicle groups (E2 group, n = 13; vehicle group, n = 11; other treatment groups, n = 6). The animals were sacrificed by C[O.sub.2] inhalation subsequent to a light [O.sub.2]/C[O.sub.2] anesthesia 24 hr after the final treatment, and necropsies were performed. A whole mount of the 4th right mammary gland was prepared, and the 4th left mammary gland was excised and fixed in 4% paraformaldehyde before embedding in paraffin. The 2nd, 3rd, and 5th mammary glands from both sides were snap-frozen in liquid nitrogen for RNA preparation.

RNA preparation. Total cytoplasmic RNA was extracted from the mammary gland tissue by the standard TRIzol[R] method (Life Technologies). The quality and the concentrations of the preparations of total RNA were determined using a NanoDrop spectrophotometer (Thermo Fisher Scientific) and an Agilent Bioanalyzer (Agilent Technologies).

mRNA microarray analyses. Total RNA (100 ng) from three rats per treatment group (vehicle, E2, 3-MC, E2 + 3-MC) that was deemed to be of good quality [RNA integrity number (RIN) [greater than or equal to] 7] was processed according to the standard Affymetrix Whole Transcript Sense Target labeling protocol. The fragmented biotin-labeled cDNA was hybridized for 16 hr to Affymetrix Gene 1.0 ST arrays and scanned on an Affymetrix Scanner 3000 7G using AGCC software (Affymetrix, Inc.). The resulting CEL files were analyzed for quality using Affymetrix Expression Console software and were then imported into GeneSpring GX11.5 (Agilent Technologies). The data were quantile-normalized using the Probe Logarithmic Intensity Error (PLIER) method and baseline-transformed to the median of the control samples. The probe sets were further filtered to exclude the bottom 20th percentile across all samples. The resulting entity list was subjected to an unpaired /'-test with Benjamini-Hochberg false discovery rate correction and a 1.5-fold filter to identify differentially expressed transcripts between conditions at a p-value < 0.05. Pathway analysis and functional annotation clustering of E2-regulated genes (p-value < 0.05) were performed using Database for Annotation, Visualization and Integrated Discovery (DAVID) 6.7 (Huang et al. 2009). All data have been deposited in the Gene Expression Omnibus (GEO, accession number GSE64636; Edgar et al. 2002).

qPCR validation of microarray data. Changes in mRNA identified by microarray were validated using five to six independent biological replicates. Reverse transcription PCR reactions were performed with 1.5 qg total RNA using Taqman[R] Reverse Transcription Reagents (Applied Biosystems) to synthesize cDNA for mRNA expression analysis. qPCR analyses were performed according to a previously described protocol (Wang WL et al. 2011) and were analyzed as follows using the ABI 7900HT Fast RealTime PCR System (Applied Biosystems): first denaturing cycle at 95[degrees]C for 3 min, then 95[degrees]C for 15 sec, 60[degrees]C for 10 sec, and 72[degrees]C for 20 sec, repeated for 40 cycles. Fluorescence was quantified at the end of the 72[degrees]C annealing step, and the amplicon specificity was confirmed by a melting curve analysis (60-95[degrees]C). Primer sequences are summarized in the Supplemental Material (Table S1). The relative mRNA amounts of target genes were calculated after normalization to an endogenous reference gene (ribosomal protein S18). The results were obtained using the [2.sup.-[DELTA][DELTA]CT] method (Pfaffl 2001) and are expressed as relative amounts of mRNA compared with those of the vehicle-treated animals.

Mammary gland whole-mount preparations. Whole-mount preparations were performed as previously described (de Assis et al. 2010). After staining with Carmine Alum (0.2% carmine, 0.5% aluminum potassium sulfate), the samples were coated with polyacrylate, placed in a water-filled petri dish, and viewed under a stereomicroscope (Stemi DRC, Carl Zeiss AG) to count the number of terminal end buds (TEBs). The TEBs of at least six animals from every treatment group were counted.

Immunohistochemistry. Dissected mammary tissue was fixed in 4% paraformaldehyde, embedded in paraffin, and sectioned at 3 [micro]m. Antigen retrieval was performed with 10 mM Tris-EDTA, pH 9 at 60[degrees]C overnight. Proteins of interest were stained using the IHC Selec[tM] Immunoperoxidase Secondary Detection System (Millipore) according to the manufacturer's protocol. Three primary antibodies [anti-progesterone receptor (PR) (1:350; Thermo Fisher Scientific), antiKi-67, a cell proliferation marker (1:150; Abcam), and anti-AHR (1:250; Abcam)] were diluted in 5% filtered skim milk powder in phosphate-buffered saline (PBS) and incubated for 1 hr at room temperature (18-20[degrees]C) in a humidified chamber. Sections were counterstained with hematoxylin (Carl Roth). The samples were visualized using a Keyence BZ-8100E (Keyence) microscope. To quantify Ki-67- and PR-positive cells, > 500 luminal epithelial cells from each of five or more animals per group were analyzed and scored using ImageJ 1.47 (Schneider et al. 2012). AHR expression was quantified by measuring the 3,3-diaminobenzidine (DAB) staining intensity of luminal epithelial cells normalized to that of the negative control group using ImageJ 1.47 (Schneider et al. 2012). For fluorescent ER[alpha] staining, tissue sections were blocked with 5% bovine serum albumin/tris-buffered saline (BSA/ TBS) + 0.1% Triton X-100 for 1 hr at room temperature in a humidified chamber. Primary anti-ER[alpha] antibody (1:250; Abcam) was diluted in 2.5% BSA/TBS, and the tissue sections were incubated overnight at room temperature. After washing with TBS, sections were incubated with CruzFluor[TM] 488 conjugated goat-anti rabbit secondary antibody (1:200 in 2.5% BSA/TBS; Santa Cruz Biotechnology) for 1 hr. Sections were mounted with Mowiol[R] (Carl Roth) and counterstained with diamidino-2-phenylindole (DAPI; 1:250; Santa Cruz). An Axiovert 100 microscope with a Colibri.2 LED illumination system (Carl Zeiss AG) was used to visualize the fluorescence-stained mammary gland epithelial cells. Magnification and exposure time were set identically to identify fluorescence intensity differences between treatment groups. The fluorescence intensity per duct was measured and normalized to that of the negative control group using ImageJ 1.47 (Schneider et al. 2012).

Statistical analysis. The data are presented as the arithmetic mean [+ or -] standard deviation (SD) for immunohistochemistry and qPCR data or as the median with percentiles (25-75%) for TEB count and immunofluorescence data. Statistical analysis included one-way analysis of variance (ANOVA) followed by the Bonferroni post hoc test to determine significant differences for the qPCR results, TEB count, immunohistochemistry, and immunofluorescence in the mammary gland. The results were considered to be statistically significant at p < 0.05.


The affinity of 3-MC for the AHR is somewhat lower than that of the prototypical ligand TCDD. The half-maximal inhibitory concentration (IC50) of 3-MC in a competitive ligand-binding assay is ~4-fold higher than that of TCDD, and the concentration of 3-MC necessary to induce Cyplal mRNA expression is between 10- and 100-fold higher (Riddick et al. 1994). We therefore opted for a much higher treatment dose of 15 mg 3-MC per kg body weight per day than the dose typically used for treatment with TCDD. This dose is similar to that used in many other studies of 3-MC as an AHR ligand (Deb and Bandiera 2010; Gottlicher and Cikryt 1987; Kondraganti et al. 2005).

Effects of 3-MC on terminal end bud development. To determine the nature of the interaction between the ligand-activated AHR and ER pathways, we assessed the effects of treating ovx rats for 3 days with E2 and 3-MC, alone or in combination, on the number of TEBs in whole-mount preparations of the mammary gland (Figure 1A). Quantitation of these data is presented in Figure 1B. The number of TEBs was significantly increased in estradiol-treated rats (46.2 [+ or -] 18.2) compared with vehicle-treated controls (8.1 [+ or -] 3.5). Differences in TEB numbers were also significant between 3-MC- (11.8 [+ or -] 2.9) and vehicle-treated controls, albeit to a far lesser extent. Co-treatment with E2 and 3-MC significantly reduced the number of TEBs compared with treatment with E2 alone (29.2 [+ or -] 9.5), although the number of TEBs remained higher than in the 3-MC--treated animals. These data suggest that the liganded AHR pathway attenuates, but does not completely block, E2 signaling mediated by the ER.

Protein levels of ER[alpha] and AHR. To determine whether the effect of 3-MC on E2 stimulation of TEB formation was the result of changing receptor levels, we assessed the status of ER[alpha] and AHR in the mammary gland. The relative mRNA levels of the ER (Esr1, Esr2) and of Ahr were not significantly different in any of the treatment groups as measured by qPCR (see Supplemental Material, Figure S1). The steady-state protein levels of ER[alpha] were significantly increased in the ductal epithelial cells after treatment with E2 alone compared with levels in the vehicle control group (Figure 2A,B). In contrast, 3-MC alone caused a significant decrease in the relative fluorescence intensity compared with that of the vehicle control, and 3-MC further abrogated the effect of E2 on ER[alpha] expression when co-administered (Figure 2B). This finding suggests that 3-MC exerts a strong anti-estrogenic effect by downregulating ER[alpha] expression. In contrast, neither 3-MC nor E2 induced any significant changes in the AHR protein in ductal epithelial cells of the mammary glands, either alone or in combination (Figure 2C; vehicle, 100 [+ or -] 17.7% relative fluorescence intensity; E2 98.9 [+ or -] 10.1% relative fluorescence intensity; 3-MC 96.8 [+ or -] 15.2% relative fluorescence intensity; E2 + 3-MC 99.3 [+ or -] 7.4% relative fluorescence intensity).

Effects of 3-MC on Ki-67 and PR expression. To investigate the cellular mechanisms responsible for the anti-estrogenic effects of 3-MC, we examined the expression of the proliferation marker Ki-67 and of PR, a classical E2-regulated target in the mammary ductal epithelium (Haslam and Shyamala 1979). As shown in Figure 3A,C, the percentage of ductal epithelial cells expressing Ki-67 increased from 1% in the vehicle-treated control animals to 44.9% after 3 days of E2 treatment. 3-MC alone did not increase Ki-67 expression, but it completely attenuated E2-induced expression of Ki-67 (4%). Similarly, treatment with E2 increased the number of PR-positive epithelial ductal cells to 53%. However, although co-administration of 3-MC significantly reduced PR-positive epithelial ductal cells to 40% (Figure 3D), it did not completely abrogate the E2-induced increase in PR levels. These data suggest that although many of the effects of 3-MC on E2 regulation of tissue growth may be attributable to its effects on ER levels, some of the physiological effects of ER are more sensitive to 3-MC than others.

Genome-wide transcriptome analysis. The effects of E2, 3-MC, and E2 + 3-MC on gene expression in the mammary gland were assessed by cDNA microarray. A 1.5-fold change filter was used to compare the changes in expression resulting from the respective treatments (3-MC, E2, E2 + 3-MC) to the vehicle controls.

Treatment with E2 differentially modulated the expression of 325 entities (Figure 4A), including 272 entities (84%) that were up-regulated and 54 (17%) that were down-regulated compared with the vehicle-treated controls. The expression change of the 15 genes that were most up-regulated by E2 ranged from 16-fold for beta-casein (Csn2) to 4-fold for kinesin family member 11 (Kif11) (Figure 4B). Although a number of genes were down-regulated by E2, the magnitude of the down-regulation was less dramatic, ranging from -4- to -2-fold for the 15 most-down-regulated genes. Pathway analyses of E2-regulated genes identified five predominant pathways [cell cycle, cell adhesion molecules, the p53 signaling pathway, pyruvate metabolism, and the insulin signaling pathway, p [less than or equal to] 0.05 (see Supplemental Material, Table S2)]. Genes involved in the control of cell division were exclusively up-regulated by E2 (see Supplemental Material, Table S2). The regulatory role of these E2 up-regulated genes in proliferative processes was confirmed by functional annotation clustering (see Supplemental Material, Figure S2). 3-MC alone modulated a total of 30 differentially expressed entities (Figure 4A), of which 25 were up-regulated and 5 were downregulated. However, only 2 of these entities (Leftyl and the mRNA for the uncharacterized protein LOC502684) were solely regulated by 3-MC, both of which were close to the 1.5 cut-off point, indicating that under these experimental conditions, 3-MC alone had minimal effects on mammary gland gene expression. Moreover, 3-MC substantially attenuated E2-mediated signaling (Figure 4C) and dampened the inductive and suppressive effects of E2 on both up-regulated and down-regulated expression of 132 of the 325 genes modulated by E2 (Figure 4D). These data show that 3-MC has a significant global antagonist action on the biological activity of E2 in the mammary gland of ovx rats.

qPCR validation of selected genes. To validate the regulation of differentially regulated genes identified in the microarray, selected genes associated with the major ontologies affected by E2 (cell cycle, cell adhesion, and p53-mediated signaling) were analyzed using qPCR. E2 had a significant effect on the expression of genes associated with cell division (Top2a, Mki67, Ccnbl, Ccnb2; Figure 5A) and cytokinesis (Kifll, Kf2c, Kif18a; Figure 5B). Although treatment with 3-MC alone had an effect on levels of Top2a, Ccnbl, and Kif2c mRNA that was far less pronounced than for treatment with E2 alone, 3-MC significantly attenuated the up-regulation of Top2a, Ccnb2, and Mki67 by E2. We also studied the effects of E2 and 3-MC on the expression of several E2-regulated genes responsible for differentiated functions of the mammary gland, including genes associated with the synthesis and secretion of milk (Areg, Csn2, Pgr, Wap, Aqp5, and Prlr), which were shown to be up-regulated by E2 in the microarray, and Retn, which was suppressed by E2 (Figure 5C,D). Although 3-MC alone had a small but statistically significant effect on Areg, Pgr, and Aqp5 expression, it significantly reduced the up-regulation of Pgr and Wap by E2.

Influence of 3-MC on 8-PN-induced effects. To determine whether the effects of 3-MC are ER-ligand dependent and whether the abrogation of estrogenic signaling by 3-MC is important in natural-compound endocrine-disruptor interactions, rats were treated with the phytoestrogen 8-PN alone or in combination with 3-MC, recapitulating the experiments described above. 8-PN significantly increased the number of TEBs, although it was clear that in this bioassay system, 8-PN was significantly less estrogenic than E2, inducing 18.7 [+ or -] 4.6 versus 46.2 [+ or -] 18.2 TEBs per gland (Figure 1B and Figure 6A). The inductive effect of 8-PN was inhibited by 50% by co-treatment with 3-MC (Figure 6A). The increase in TEBs in response to 8-PN was reflected in the increase in the percentage of Ki-67-positive cells, which was substantially lower than with E2 treatment (8.1 [+ or -] 4.1% vs. 44.9 [+ or -] 14.7%, respectively), confirming the weaker estrogenic potency of 8-PN. Co-treatment with 3-MC effectively blocked the 8-PN-induced increase in proliferating cells, but statistical significance was not achieved (p = 0.05891, Figure 6B). To investigate the effects on gene expression of 8-PN alone and in co-treatment with 3-MC, we chose genes that were identified in earlier experiments as being highly regulated by E2 (Areg, Csn2, Pgr) as well as genes associated with proliferation (Kif, Mki67; Figure 6C). Although 8-PN weakly induced the expression of some of the E2 target genes (Kif11, Kif2c, Kif18a, Csn2), a significant counteracting effect of 3-MC on 8-PN-induced gene expression was observed for Csn2, Kif18a, and Kif11, in which the relative expression of the mRNA was significantly abrogated after co-treatment. However, some of the gene expression patterns induced by 8-PN were different from those induced by E2 because 8-PN decreased Mki67 expression and had no significant effects on Areg or Pgr expression.


Interaction of xenobiotics with the hormonal system in the mammary gland is of great relevance regarding cancer risks and other syndromes whose etiologies are associated with hormonal interferences. In the present study, we investigated the cross-talk between ER-and AHR-mediated signaling processes in the female rat mammary gland using an ovariectomized rat mammary gland model system. This is a very sensitive model system for examining the physiological effects of E2 and the interactions between E2 and environmental AHR ligands such as TCDD and 3-MC.

The data presented herein are in line with the large body of literature demonstrating antiestrogenic effects of AHR ligands in cell culture (Gierthy et al. 1987; Safe and Krishnan 1995; Ueng et al. 2004; Wang F et al. 1998; Wormke et al. 2000). We demonstrated that 3-MC has inhibitory effects on the expression of a significant proportion of E2-modulated genes and has pronounced effects on physiological responses to E2. Within the last 15 years, there have been several reports of the inhibitory effects of TCDD on mammary gland development in both animals (Fenton et al. 2002; Vorderstrasse et al. 2004) and humans (Den Hond et al. 2002). In addition, animal studies (Collins et al. 2009; Vorderstrasse et al. 2004) and studies using primary mammary epithelial cells and HC-11 cells (Basham et al. 2015) suggested that AHR activation has a negative impact on milk production, resulting in the inability of mice to nutritionally support their offspring (Vorderstrasse et al. 2004). The inhibition of E2-induced development of TEBs, cell proliferation, up-regulation of the cell cycle, and proliferation-related pathways that we observed in response to 3-MC treatment suggests that these effects are independent of the specific AHR ligand and could therefore also be caused by the much more abundant PAHs. Furthermore, our data suggest that the adverse effects of AHR ligands on mammary gland development are most likely based on their ER-antagonistic properties. These data also offer an explanation for the observed decrease of mammary tumors in female rats after long-term treatment with TCDD (Kociba et al. 1978) and for the wellknown inhibitory properties of exogenous AHR ligands on rodent mammary gland tumors and metastasis development (Lubet et al. 2011; Safe 2001; Wang T et al. 2011). Given the similarity between the development and carcinogenesis of rodent and human mammary glands (Rudel et al. 2011), the antiestrogenic effects of AHR-mediated signaling may at least partially explain the increased overall survival and distant metastasis-free survival in hormone-dependent ER-positive breast cancers in human patients with elevated AHR expression (O'Donnell et al. 2014; Saito et al. 2013).

There are several mechanisms that might explain these ER-antagonistic effects. Many AHR ligands, among them 3-MC, have been shown to directly interact with ERs (Abdelrahim et al. 2006; Liu et al. 2006). In the case of 3-MC, this interaction is very weak but measurable. This affinity for both ERs may lead to activation of ERs in some tissues but to antagonistic effects in others. Notably, in mammary gland-derived HC11 cells, 3-MC acts as an AHR-independent ER[alpha] antagonist (Swedenborg et al. 2008), and this is therefore also likely to be the case in the mammary gland. In contrast, TCDD displays similar anti-estrogenic properties, although its affinity for ER[alpha] and ER[beta] is even lower and it is typically tested at much lower concentrations than 3-MC owing to its persistency. In the present study, only the expression changes of a subset of E2-regulated genes were blocked by 3-MC treatment. It is therefore likely that additional mechanisms are involved in mediating the anti-estrogenic response of AHR ligands in general and of 3-MC in particular. Firstly, AHR ligands alter hepatic E2 metabolism in female rats through the activation of several hepatic P450 cytochromes, increasing conversion of E2 to 2-hydroxyestradiol and 7a-hydroxyestradiol and thereby decreasing its bioavailability (Suchar et al. 1996). Secondly, the AHR has been identified as a component of a cullin 4B ubiquitin ligase complex (CUL4Bahr) (Ohtake et al. 2007), and in the rat uterus, activation of the AHR by 3-MC and other ligands of the receptor results in ubiquitination and proteasomal degradation of the ER and other steroid receptors (Wormke et al. 2003). A decrease in the level of the ligand (due to metabolism) and/or the receptor (due to degradation) would be anticipated to have global effects on E2-dependent gene expression in the mammary gland. Although 3-MC had significant inhibitory effects on E2-mediated modulation of many genes in the mammary gland (132/325, 41%), a great proportion (193/325, 59%) of the E2-responsive genes were not affected by 3-MC (Figure 4). This finding indicates that the effects of 3-MC on mammary gland physiology and gene expression cannot be solely (or even primarily) attributed to its effects on hepatic metabolism or on the stability of the estrogen receptor. This idea is also supported by the observed effects of 3-MC on the estrogenic actions of 8-PN, a naturally occurring, plant-derived ER ligand (Helle et al. 2014; Kitaoka et al. 1998; Milligan et al. 1999). Even though 8-PN is a weak estrogen and is metabolized differently in the liver (Guo et al. 2006; Keiler et al. 2015), the effects of 3-MC on 8-PN-mediated gene expression partially mirror effects observed with E2. Importantly, co-treatment with 3-MC also counteracted some of the effects of 8-PN, suggesting that the inhibitory effects of 3-MC are independent of which ligand is bound to the ER.


Our data give a detailed account of the in vivo effects of E2 and 3-MC on gene expression and on development of mammary glands, and they demonstrate that AHR ligands such as 3-MC are anti-estrogenic with regard to many E2-regulated genes in the mammary gland. Almost no E2-independent effects of 3-MC on gene expression were observed, indicating that interaction with ERs is the predominant mode of action of AHR in the mammary gland. This finding helps to explain the adverse effects of AHR ligands on mammary gland development and underlines the potential of AHR as a breast cancer therapy target. We identified degradation of ER[alpha] as another putative mechanism by which 3-MC and possibly other PAHs inhibit ER signaling in vivo. Moreover, changes in gene expression caused by the phytoestrogen 8-PN were also reduced following 3-MC treatment, but further studies will be required to assess the importance of the interactions between ERs and AHR with regard to different endogenous, exogenous, nutrition-derived, and synthetic ER ligands in vivo.

Address correspondence to J. Helle, Institute of Zoology, Molecular Cell Physiology and Endocrinology, Technische Universitat Dresden, Zellescher Weg 20b, 01062 Dresden, Germany, Telephone: (49) 351-46331942. E-mail: Janina.

Supplemental Material is available online (http://

We thank F. Moller (Institute of Zoology, Technische Universitat Dresden, Germany) and the facility members of S. Chittur (Department of Biomedical Sciences, University at Albany, State University of New York, United States) for their help and technical support.

This work was funded by the Deutsche Forschungsgemeinschaft (KR 3768/2-1) and the TU Dresden Forschungspool (TU Dresden Research Pool).

The authors declare they have no actual or potential competing financial interests.

Received: 6 January 2015; Accepted: 10 September 2015; Advance Publication: 15 September 2015; Final Publication: 1 May 2016.


Abdelrahim M, Ariazi E, Kim K, Khan S, Barhoumi R, Burghardt R, et al. 2006. 3-Methylcholanthrene and other aryl hydrocarbon receptor agonists directly activate estrogen receptor a. Cancer Res 66(4):2459-2467; doi:10.1158/0008-5472.CAN-05-3132.

Basham KJ, Leonard CJ, Kieffer C, Shelton DN, McDowell ME, Bhonde VR, et al. 2015. Dioxin exposure blocks lactation through a direct effect on mammary epithelial cells mediated by the aryl hydrocarbon receptor repressor. Toxicol Sci 143(1):36-45; doi:10.1093/toxsci/kfu203.

Beischlag TV, Luis Morales J, Hollingshead BD, Perdew GH. 2008. The aryl hydrocarbon receptor complex and the control of gene expression. Crit Rev Eukaryot Gene Expr 18(3):207-250.

Beischlag TV, Perdew GH. 2005. ER[alpha]-AHRARNT protein-protein interactions mediate estradiol-dependent transrepression of dioxininducible gene transcription. J Biol Chem 280(22):21607-21611; doi:10.1074/jbc.C500090200.

Chen B, Hou ZH, Dong Z, Li CD. 2015. Crocetin down-regulates the proinflammatory cytokines in methylcholanthrene-induced rodent tumor model and inhibits COX-2 expression in cervical cancer cells. Biomed Res Int 2015:829513; doi:10.1155/2015/829513.

Collins LL, Lew BJ, Lawrence BP. 2009. TCDD exposure disrupts mammary epithelial cell differentiation and function. Reprod Toxicol 28(1):11-17; doi:10.1016/j.reprotox.2009.02.013.

de Assis S, Warri A, Cruz MI, Hilakivi-Clarke L. 2010. Changes in mammary gland morphology and breast cancer risk in rats. J Vis Exp 44:2260; doi:10.3791/2260.

Deb S, Bandiera SM. 2010. Characterization of a new cytochrome P450 enzyme, CYP2S1, in rats: its regulation by aryl hydrocarbon receptor agonists. Toxicology 267(1-3):91-98; doi:10.1016/j. tox.2009.10.025.

Denison MS, Pandini A, Nagy SR, Baldwin EP, Bonati L. 2002. Ligand binding and activation of the Ah receptor. Chem Biol Interact 141(1-2):3-24.

Edgar R, Domrachev M, Lash AE. 2002. Gene expression omnibus: NCBI gene expression and hybridization array data repository. Nucleic Acids Res 30(1):207-210; doi:10.1093/nar/30.1.207.

Fenton SE, Hamm JT, Birnbaum LS, Youngblood GL. 2002. Persistent abnormalities in the rat mammary gland following gestational and lactational exposure to 2,3,7,8-tetrachlorodibenzo-p-dioxin (TCDD). Toxicol Sci 67(1):63-74; doi:10.1093/toxsci/67.1.63.

Gester S, Metz P, Zierau O, Vollmer G. 2001. An efficient synthesis of the potent phytoestrogens 8-prenylnaringenin and 6-(1,1-dimethylallyl)naringenin by europium(III)-catalyzed Claisen rearrangement. Tetrahedron 57(6):1015-1018; doi:10.1016/ S0040-4020(00)01078-4.

Gierthy JF, Lincoln DW, Gillespie MB, Seeger JI, Martinez HL, Dickerman HW, et al. 1987. Suppression of estrogen-regulated extracellular tissue plasminogen activator activity of MCF-7 cells by 2,3,7,8-tetrachlorodibenzo-p-dioxin. Cancer Res 47(23):6198-6203.

Gottlicher M, Cikryt P. 1987. Induction of the aromatic hydrocarbon receptor by frans-4-acetylaminostilbene in rat liver. Comparison with other aromatic amines. Carcinogenesis 8(7):1021-1023.

Guo J, Nikolic D, Chadwick LR, Pauli GF, van Breemen RB. 2006. Identification of human hepatic cytochrome P450 enzymes involved in the metabolism of 8-prenylnaringenin and isoxanthohumol from hops (Humulus lupulus L.). Drug Metab Dispos 34(7):1152-1159; doi:10.1124/dmd.105.008250.

Hankinson O. 1995. The aryl hydrocarbon receptor complex. Annu Rev Pharmacol Toxicol 35(1):307-340; doi:10.1146/

Haslam SZ, Shyamala G. 1979. Effect of oestradiol on progesterone receptors in normal mammary glands and its relationship with lactation. Biochem J 182(1):127-131.

Helle J, Kraker K, Bader MI, Keiler AM, Zierau O, Vollmer G, et al. 2014. Assessment of the proliferative capacity of the flavanones 8-prenylnaringenin, 6-(1.1-dimethylallyl)naringenin and naringenin in MCF-7 cells and the rat mammary gland. Mol Cell Endocrinol 392(1-2):125-135; doi:10.1016/j. mce.2014.05.014.

Hernandez-Ochoa I, Karman BN, Flaws JA. 2009. The role of the aryl hydrocarbon receptor in the female reproductive system. Biochem Pharmacol 77(4):547-559; doi:10.1016/j.bcp.2008.09.037.

Den Hond E, Roels HA, Hoppenbrouwers K, Nawrot T, Thijs L, Vandermeulen C, et al. 2002. Sexual maturation in relation to polychlorinated aromatic hydrocarbons: Sharpe and Skakkebaek's hypothesis revisited. Environ Health Perspect 110:771-776.

Huang da W, Sherman BT, Lempicki RA. 2009. Systematic and integrative analysis of large gene lists using DAVID bioinformatics resources. Nat Protoc 4(1):44-57; doi:10.1038/nprot.2008.211.

Hushka LJ, Williams JS, Greenlee WF. 1998. Characterization of 2,3,7,8-tetrachlorodibenzofurandependent suppression and AH receptor pathway gene expression in the developing mouse mammary gland. Toxicol Appl Pharmacol 152(1):200-210; doi:10.1006/taap.1998.8508.

Keiler AM, Dorfelt P, Chatterjee N, Helle J, Bader MI, Vollmer G, et al. 2015. Assessment of the effects of naringenin-type flavanones in uterus and vagina. J Steroid Biochem Mol Biol 145:49-57; doi:10.1016/j. jsbmb.2014.10.001.

Kerkvliet NI. 2002. Recent advances in understanding the mechanisms of TCDD immunotoxicity. Int Immunopharmacol 2(2-3):277-291.

Kitaoka M, Kadokawa H, Sugano M, Ichikawa K, Taki M, Takaishi S, et al. 1998. Prenylflavonoids: a new class of non-steroidal phytoestrogen (part 1). Isolation of 8-isopentenylnaringenin and an initial study on its structure-activity relationship. Planta Med 64(6):511-515; doi:10.1055/s-2006-957504.

Kociba RJ, Keyes DG, Beyer JE, Carreon RM, Wade CE, Dittenber DA, et al. 1978. Results of a two-year chronic toxicity and oncogenicity study of 2,3,7,8-tetrachlorodibenzo-p-dioxin in rats. Toxicol Appl Pharmacol 46(2):279-303; doi:10.1016/0041-008X(78)90075-3.

Kondraganti SR, Muthiah K, Jiang W, Barrios R, Moorthy B. 2005. Effects of 3-methylcholanthrene on gene expression profiling in the rat using cDNA microarray analyses. Chem Res Toxicol 18(11):1634-1641; doi:10.1021/tx050085n.

Larsen MC, Angus WG, Brake PB, Eltom SE, Sukow KA, Jefcoate CR. 1998. Characterization of CYP1B1 and CYP1A1 expression in human mammary epithelial cells: role of the aryl hydrocarbon receptor in polycyclic aromatic hydrocarbon metabolism. Cancer Res 58(11):2366-2374.

Le Provost F, Riedlinger G, Hee Yim S, Benedict J, Gonzalez FJ, Flaws J, etal. 2002. The aryl hydrocarbon receptor (AhR) and its nuclear translocator (Arnt) are dispensable for normal mammary gland development but are required for fertility. Genesis 32(3):231-239.

Liu S, Abdelrahim M, Khan S, Ariazi E, Jordan VC, Safe S. 2006. Aryl hydrocarbon receptor agonists directly activate estrogen receptor a in MCF-7 breast cancer cells. Biol Chem 387(9):1209-1213; doi:10.1515/BC.2006.149.

Lubet RA, Heckman BM, De Flora SL, Steele VE, Crowell JA, Juliana MM, et al. 2011. Effects of 5,6-benzoflavone, indole-3-carbinol (I3C) and diindolylmethane (DIM) on chemically-induced mammary carcinogenesis: is DIM a substitute for I3C? Oncol Rep 26(3):731-736; doi:10.3892/or.2011.1316.

Matsumura F, Vogel CF. 2006. Evidence supporting the hypothesis that one of the main functions of the aryl hydrocarbon receptor is mediation of cell stress responses. Biol Chem 387(9):1189-1194; doi:10.1515/BC.2006.146.

Matthews J, Wihlen B, Thomsen J, Gustafsson JA. 2005. Aryl hydrocarbon receptor-mediated transcription: ligand-dependent recruitment of estrogen receptor a to 2,3,7,8-tetrachlorodibenzo-p-dioxinresponsive promoters. Mol Cell Biol 25(13):5317-5328; doi:10.1128/MCB.25.13.5317-5328.2005.

Milligan SR, Kalita JC, Heyerick A, Rong H, De Cooman L, De Keukeleire D. 1999. Identification of a potent phytoestrogen in hops (Humulus lupulus L.) and beer. J Clin Endocrinol Metab 84(6):2249-2252.

Mimura J, Fujii-Kuriyama Y. 2003. Functional role of AhR in the expression of toxic effects by TCDD. Biochim Biophys Acta 1619(3):263-268.

O'Donnell EF, Koch DC, Bisson WH, Jang HS, Kolluri SK. 2014. The aryl hydrocarbon receptor mediates raloxifene-induced apoptosis in estrogen receptornegative hepatoma and breast cancer cells. Cell Death Dis 5:e1038; doi:10.1038/cddis.2013.549.

Ohtake F, Baba A, Fujii-Kuriyama Y, Kato S. 2008. Intrinsic AhR function underlies cross-talk of dioxins with sex hormone signalings. Biochem Biophys Res Commun 370(4):541-546; doi:10.1016/j.bbrc.2008.03.054.

Ohtake F, Baba A, Takada I, Okada M, Iwasaki K, Miki H, et al. 2007. Dioxin receptor is a ligand-dependent E3 ubiquitin ligase. Nature 446(7135):562-566; doi:10.1038/nature05683.

Ohtake F, Takeyama K, Matsumoto T, Kitagawa H, Yamamoto Y, Nohara K, et al. 2003. Modulation of oestrogen receptor signalling by association with the activated dioxin receptor. Nature 423(6939):545-550; doi:10.1038/nature01606.

Pfaffl MW. 2001. A new mathematical model for relative quantification in real-time RT--PCR. Nucleic Acids Res 29(9):e45; doi:10.1093/nar/29.9.e45.

Poellinger L. 2000. Mechanistic aspects--the dioxin (aryl hydrocarbon) receptor. Food Addit Contam 17(4):261-266; doi:10.1080/026520300283333.

Puga A, Ma C, Marlowe JL. 2009. The aryl hydrocarbon receptor cross-talks with multiple signal transduction pathways. Biochem Pharmacol 77(4):713-722; doi:10.1016/j.bcp.2008.08.031.

Riddick DS, Huang Y, Harper PA, Okey AB. 1994. 2,3,7,8-Tetrachlorodibenzo-p-dioxin versus 3-methylcholanthrene: comparative studies of Ah receptor binding, transformation, and induction of CYP1A1. J Biol Chem 269(16):12118-12128.

Rudel RA, Fenton SE, Ackerman JM, Euling SY, Makris SL. 2011. Environmental exposures and mammary gland development: state of the science, public health implications, and research recommendations. Environ Health Perspect 119:1053-1061; doi:10.1289/ehp.1002864.

Rymaszewski AL, Tate E, Yimbesalu JP, Gelman AE, Jarzembowski JA, Zhang H, et al. 2014. The role of neutrophil myeloperoxidase in models of lung tumor development. Cancers (Basel) 6(2):1111-1127; doi:10.3390/cancers6021111.

Safe S. 2001. Molecular biology of the Ah receptor and its role in carcinogenesis. Toxicol Lett 120(1-3):1-7.

Safe S, Krishnan V. 1995. Chlorinated hydrocarbons: estrogens and antiestrogens. Toxicol Lett 82-83:731-736.

Saito R, Miki Y, Hata S, Takagi K, Iida S, Oba Y, et al. 2013. Aryl hydrocarbon receptor in breast cancer-a newly defined prognostic marker. Horm Cancer 5(1):11-21; doi:10.1007/s12672-013-0160-z.

Schneider CA, Rasband WS, Eliceiri KW. 2012. NIH Image to ImageJ: 25 years of image analysis. Nat Methods 9(7):671-675.

Shanle EK, Xu W. 2011. Endocrine disrupting chemicals targeting estrogen receptor signaling: identification and mechanisms of action. Chem Res Toxicol 24(1):6-19; doi:10.1021/tx100231n.

Suchar LA, Chang RL, Thomas PE, Rosen RT, Lech J, Conney AH. 1996. Effects of phenobarbital, dexamethasone, and 3-methylcholanthrene administration on the metabolism of 17 beta-estradiol by liver microsomes from female rats. Endocrinology 137(2):663-676; doi:10.1210/endo.137.2.8593816.

Swedenborg E, Pongratz I. 2010. AhR and ARNT modulate ER signaling. Toxicology 268(3):132-138; doi:10.1016/j.tox.2009.09.007.

Swedenborg E, Ruegg J, Hillenweck A, Rehnmark S, Faulds MH, Zalko D, et al. 2008. 3-Methylcholanthrene displays dual effects on estrogen receptor (ER) [alpha] and ER[beta] signaling in a cell-type specific fashion. Mol Pharmacol 73(2):575-586; doi:10.1124/mol.107.036384.

Ueng TH, Hung CC, Wang HW, Chan PK. 2004. Effects of amitraz on cytochrome P450-dependent monooxygenases and estrogenic activity in MCF-7 human breast cancer cells and immature female rats. Food Chem Toxicol 42(11):1785-1794; doi:10.1016/j. fct.2004.06.010.

Vorderstrasse BA, Fenton SE, Bohn AA, Cundiff JA, Lawrence BP. 2004. A novel effect of dioxin: exposure during pregnancy severely impairs mammary gland differentiation. Toxicol Sci 78(2):248-257; doi:10.1093/toxsci/kfh062.

Wang F, Hoivik D, Pollenz R, Safe S. 1998. Functional and physical interactions between the estrogen receptor Sp1 and nuclear aryl hydrocarbon receptor complexes. Nucleic Acids Res 26(121:3044-3052.

Wang T, Wyrick KL, Meadows GG, Wills TB, Vorderstrasse BA. 2011. Activation of the aryl hydrocarbon receptor by TCDD inhibits mammary tumor metastasis in a syngeneic mouse model of breast cancer. Toxicol Sci 124(21:291-298; doi:10.1093/toxsci/kfr247.

Wang WL, Chatterjee N, Chittur SV, Welsh J, Tenniswood MP. 2011. Effects of 1a,25 dihydroxyvitamin D3 and testosterone on miRNA and mRNA expression in LNCaP cells. Mol Cancer 10:58; doi:10.1186/1476-4598-10-58.

Whitlock JP Jr, Okino ST, Dong L, Ko HP, Clarke-Katzenberg R, Ma Q, et al. 1996. Cytochromes P450 5: induction of cytochrome P4501A1: a model for analyzing mammalian gene transcription. FASEB J 10(81:809-818.

Wormke M, Stoner M, Saville B, Walker K, Abdelrahim M, Burghardt R, et al. 2003. The aryl hydrocarbon receptor mediates degradation of estrogen receptor a through activation of proteasomes. Mol Cell Biol 23(61:1843-1855.

Wormke M, Stoner M, Saville B, Safe S. 2000. Crosstalk between estrogen receptor a and the aryl hydrocarbon receptor in breast cancer cells involves unidirectional activation of proteasomes. FEBS Lett 478(1-21:109-112.

Zierau O, Kretzschmar G, Moller F, Weigt C, Vollmer G. 2008. Time dependency of uterine effects of naringenin type phytoestrogens in vivo. Mol Cell Endocrinol 294(1-21:92-99; doi:10.1016/j. mce.2008.08.008.

Janina Helle, (1) Manuela I. Bader, (1) Annekathrin M. Keiler, (1) Oliver Zierau, (1) Gunter Vollmer, (1) Sridar V. Chittur, (2) Martin Tenniswood, (2) and Georg Kretzschmar (1)

(1) Institute of Zoology, Molecular Cell Physiology and Endocrinology, Technische Universitat Dresden, Dresden, Germany; (2) Department of Biomedical Sciences, University at Albany, State University of New York, Albany, New York, USA

Caption: Figure 1. Effects of 17[beta]-estradiol (E2) and 3-methylcholanthrene (3-MC), alone and in combination, on terminal end bud (TEB) formation in ovariectomized (ovx) rats. Ovx rats were treated with E2, 3-MC, E2 + 3-MC, or vehicle control for 3 days. Mammary gland whole mounts were prepared and stained as described in "Methods." (4) Representative TEB formation in mammary whole mounts from each treatment group. Arrows highlight TEBs. Magnification scale: 500 [micro]m. (B) Quantification of the effects of E2 and 3-MC, alone and in combination, on TEB formation. Diamonds represent individual animals; boxes indicate 25th to 75th percentiles, and the horizontal lines indicate the median. The whiskers indicate the highest and the lowest measured values partitioned by the median. * Significant differences (p < 0.05) from vehicle control [one-way analysis of variance (ANOVA)]. #Significant differences (p < 0.05) from E2 treatment alone (one-way ANOVA).

Caption: Figure 2. Effects of 17[beta]-estradiol (E2) and 3-methylcholanthrene (3-MC), alone and in combination, on estrogen receptor alpha (ER[alpha]) and aryl hydrocarbon receptor (AHR) status in mammary glands from ovariectomized (ovx) rats. Ovx rats were treated with E2, 3-MC, E2 + 3-MC, or vehicle control for 3 days. (4) Representative expression of ER[alpha] in mammary glands from each treatment group. Tissue sections were prepared for immunofluorescence microscopy as described in "Methods." Magnification scale: 30 [micro]m. DAPI, diamidino-2-phenylindole. (B) Quantification of the effects of E2 and 3-MC, alone and in combination, on ER[alpha] expression in the mammary glands of 6 animals per treatment group. Fluorescence intensity per duct was measured as described in "Methods" and normalized to the vehicle control. Diamonds represent individual ducts; boxes show the 25th and 75th percentiles, and the horizontal lines indicate the median. The whiskers mark the standard deviation for each treatment group. (C) Representative immunohistochemical staining for AHR in mammary gland ducts labeled with an antibody against AHR for each treatment group. Paraffin-embedded sections were prepared for immunohistochemistry using 3,3'-diaminobenzidine (DAB) as described in "Methods." Magnification scale: 50 [micro]m.

* Significant differences (p < 0.05) from vehicle control [one-way analysis of variance (ANOVA)]. #Significant differences (p < 0.05) from E2 treatment alone (one-way ANOVA).

[dagger]Significant differences (p < 0.05) from 3-MC treatment alone (one-way ANOVA).

Caption: Figure 3. Ki-67 and progesterone receptor (PR) protein expression in the mammary gland. Ovariectomized (ovx) rats were treated with 17[beta]-estradiol (E2), 3-methylcholanthrene (3-MC), E2 + 3-MC, or vehicle control for 3 days. Paraffin-embedded sections were prepared for immunohistochemistry using 3,3'-diaminobenzidine (DAB) as described in "Methods." Paraffin-embedded sections of rat mammary glands from each treatment group were stained with DAB using antibodies against Ki-67 (4) or PR (6) and counterstained with hematoxylin. Magnification scale: 50 [micro]m. (C,D) Quantification of the effects of E2 and 3-MC, alone and in combination, on Ki-67 and PR protein levels. The number of positively stained epithelial cells were counted and normalized to the total number of epithelial cells; [greater than or equal to] 500 cells were evaluated per animal, and five to six animals were used per treatment group. Data are presented as the arithmetic mean [+ or -] SD.

* Significant differences (p < 0.05) from vehicle control [one-way analysis of variance (ANOVA)]. #Significant differences (p < 0.05) from E2 treatment alone (one-way ANOVA).

Caption: Figure 4. Genome-wide transcriptome analysis of the effects of 17[beta]-estradiol (E2) and 3-methylcholanthrene (3-MC), alone and in combination, in mammary glands from ovariectomized (ovx) rats. Ovx rats were treated for 3 days with E2, 3-MC, E2 + 3-MC, or vehicle control. RNA was extracted from mammary glands from each treatment group, and global gene expression changes were analyzed by microarray as described in "Methods." Three independent biological replicates were interrogated for each treatment group. (4) Venn diagram illustrating the number of entities modulated by each treatment and overlap in target genes between treatment groups. Fold change (FC) [greater than or equal to] 1.5 compared with the vehicle control. (B) FC of all entities modulated by entities from the mammary gland of E2 or E2 + 3-MC treated rats compared with vehicle-treated control rats. (C) Comparison of the FC of the 15 most up- and down-regulated genes by E2 and E2 + 3-MC treatment. (D) Interaction analysis for E2- and 3-MC-mediated gene expression. The FC of entities regulated by E2 + 3-MC and E2 are compared. The relative expression values of the E2 treatment group were set to 0. FC [greater than or equal to] 1.5 compared with the E2 group.

Caption: Figure 5. Expression of selected genes in mammary glands in ovariectomized (ovx) rats in response to 170-estradiol (E2) and 3-methylcholanthrene (3-MC), alone and in combination. Ovx rats were treated for 3 days with E2, 3-MC, E2 + 3-MC, or vehicle control. RNA was extracted from the mammary glands, and expression of individual genes was assessed using quantitative polymerase chain reaction (qPCR) as described in "Methods." (4) Genes associated with cell cycle and proliferation; (B) genes associated with cytokinesis; (C) classical E2-responsive genes; (D) genes associated with differentiated mammary gland function. Data are presented as fold change, mean [+ or -] SD, for each treatment group relative to vehicle-treated controls. Five to six animals per treatment group were analyzed. *Significant differences (p < 0.05) from vehicle control [one-way analysis of variance (ANOVA)]. #Significant differences (p < 0.05) from E2 treatment alone (one-way ANOVA).

Caption: Figure 6. Effect of 8-prenylnaringenin (8-PN) and 3-methylcholanthrene (3-MC), alone and in combination, on terminal end bud (TEB) number, Ki-67 staining, and mRNA expression in mammary glands from ovariectomized (ovx) rats. Ovx rats were treated for 48 hr with 3-MC, 8-PN, 8-PN + 3-MC, or vehicle control as described in "Methods." (4) Quantitation of the effects of 8-PN and 3-MC, alone and in combination, on TEB formation in mammary whole mounts. Mammary gland whole mounts were prepared, stained, and quantitated as described in "Methods." Diamonds represent individual animals; boxes indicate the 25th and 75th percentiles, and the horizontal lines indicate the median. The whiskers indicate the highest and the lowest measured values for each treatment group. (B) Ki-67 expression in mammary glands from ovx rats treated with 8-PN or 3-MC alone or in combination. Paraffin-embedded sections of rat mammary glands from each treatment group were stained with 3,3'-diaminobenzidine (DAB) using antibodies against Ki-67 and were counterstained with hematoxylin. The number of positively stained epithelial cells were counted and normalized to the total number of epithelial cells; > 500 cells were evaluated per animal, and five to six animals were used per treatment group. Data are presented as the arithmetic mean [+ or -] SD. (C) Quantitative polymerase chain reaction (qPCR) analysis of selected genes in mammary glands from ovx rats treated with 8-PN or 3-MC alone or in combination. The results are presented as the mean [+ or -] SD, n = 5-6.

* Significant differences (p < 0.05) from vehicle control [one-way analysis of variance (ANOVA)]. #Significant differences (p < 0.05) from 8-PN treatment alone (one-way ANOVA).


Please note: Illustration(s) are not available due to copyright restrictions.
COPYRIGHT 2016 National Institute of Environmental Health Sciences
No portion of this article can be reproduced without the express written permission from the copyright holder.
Copyright 2016 Gale, Cengage Learning. All rights reserved.

Article Details
Printer friendly Cite/link Email Feedback
Title Annotation:Research
Author:Helle, Janina; Bader, Manuela I.; Keiler, Annekathrin M.; Zierau, Oliver; Vollmer, Gunter; Chittur,
Publication:Environmental Health Perspectives
Article Type:Report
Geographic Code:4EUGE
Date:May 1, 2016
Previous Article:Developmental effects of the ToxCast[TM] phase I and phase II chemicals in Caenorhabditis elegans and corresponding responses in zebrafish, rats, and...
Next Article:E-waste and harm to vulnerable populations: a growing global problem.

Terms of use | Privacy policy | Copyright © 2022 Farlex, Inc. | Feedback | For webmasters |