Can Breast Tumors Affect the Oxidative Status of the Surrounding Environment? A Comparative Analysis among Cancerous Breast, Mammary Adjacent Tissue, and Plasma

Panis, C.; Victorino, V. J.; Herrera, A. C. S. A.; Cecchini, A. L.; Simão, A. N. C.; Tomita, L. Y.; Cecchini, R.

doi:https://doi.org/10.1155/2016/6429812

Oxidative Medicine and Cellular Longevity

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Abstract Introduction Methods Results Discussion Acknowledgments References Copyright Related Articles

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Oxidative Stress and Cancer: Advances and Challenges

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Research Article | Open Access

Volume 2016 | Article ID 6429812 | https://doi.org/10.1155/2016/6429812

Can Breast Tumors Affect the Oxidative Status of the Surrounding Environment? A Comparative Analysis among Cancerous Breast, Mammary Adjacent Tissue, and Plasma

C. Panis,¹V. J. Victorino,²A. C. S. A. Herrera,³A. L. Cecchini,⁴A. N. C. Simão,⁵L. Y. Tomita,⁶and R. Cecchini⁴

Academic Editor: Manoj K. Pandey

Received22 May 2015

Revised04 Aug 2015

Accepted12 Aug 2015

Published30 Nov 2015

Abstract

In this paper, we investigated the oxidative profile of breast tumors in comparison with their normal adjacent breast tissue. Our study indicates that breast tumors present enhanced oxidative/nitrosative stress, with concomitant augmented antioxidant capacity when compared to the adjacent normal breast. These data indicate that breast cancers may be responsible for the induction of a prooxidant environment in the mammary gland, in association with enhanced TNF-α and nitric oxide.

1. Introduction

Redox imbalance is a process reported in most of the chronic diseases [1]. The constant activity of reactive species (RS) on lipids, DNA, and proteins promotes critical modifications in cell physiology [2], which can interfere with its normal functioning under chronic inflammatory conditions, such as cancer [3].

Cancer cells constantly experience moderate to high levels of oxidative stress, but curiously moderate to high oxidative stress does not cause immediate cell death [4]. This fact indicates that cancer cells are able to overcome and adapt against redox changes. The sustained oxidative stress promoted during chronic inflammation supports pivotal events to cancer survival, including most of the hallmarks of cancer. This fact has been associated with aberrant activation of transcription factors, induction of protooncogenes, and cumulative acquisition of mutations, which perpetuates the genomic instability of cancer cells [5].

Tumors with enhanced proliferative capacity, as breast cancer, produce high levels of RS during their chronic cycles of ischemia, reperfusion, and angiogenesis, resulting in exceeding growth signaling [6]. It is reported that DNA obtained from breast carcinomas presents greater oxidative damage than the adjacent nontumoral breast [7], suggesting that the tumor cells are more exposed to in situ oxidative stress than the proximal or distant nontumoral tissues. On the other hand, this fact suggests that cancer can potentially induce oxidative damage in surrounding normal cells.

Therefore, nontransformed epithelial cells located adjacently to the tumoral tissue may experience variable concentrations of RS generated by the constitutive activation of mitogenic pathways arising from surrounding tumor cells [8]; however, the impact of this event on the homeostasis of nontumoral adjacent cells is unclear. What is known so far is that tumors are “oxidatively stressed” and that in some extension it could be related with the systemic redox changes reported in patients bearing breast tumors [9–11].

Although growing evidence highlights the occurrence of persistent oxidative stress in breast tumors, most of studies have not focused on reporting the redox modifications of breast cancer regarding its healthy counterpart tissue and whether there is a relationship between the tumor oxidative status and the systemic redox profiling. In this context, we proposed to map the oxidative and inflammatory profiles of fresh nonfixed breast tumors and their paired adjacent mammary nontumoral tissue, as well as their respective plasma. To reach these goals, we designed our analysis employing high-sensitivity oxidative stress approaches to investigate the functional redox changes that occurred in tumor microenvironment and its correlation with the circulating levels of proinflammatory/oxidative mediators.

2. Material and Methods

2.1. Study Design

A series of 321 women with breast cancer were screened from March 2011 to December 2012 at Londrina Cancer Institute, Londrina, Paraná, Brazil. A total of 50 women were included based on the inclusion and exclusion criteria. Inclusion criteria embraced women bearing unilateral tumor with histopathological diagnosis of primary ductal infiltrative carcinoma of the breast, before starting the chemotherapeutic regimen. Exclusion criteria included current smoking, hepatic, cardiac, or renal dysfunction, obesity, use of drugs, hypertension, autoimmune disorders, and diabetes, among other chronic conditions.

Adjacent mammary tissue and tumoral tissue were surgically resected at the moment of tumor withdrawal according to standard procedures, before chemotherapy starting. The adjacent tissue was collected from the most distant point in relation to the tumoral tissue (3 to 4 cm of distance from the macroscopic tumor). Adjacent breast was confirmed as nontumoral by conventional histopathological analysis. Heparinized blood was further collected for analysis. Samples were kept frozen at −86°C until analysis, by at most 2 weeks.

All recommendations of the Reporting Recommendations for Tumor Marker Prognostic Studies (REMARK) criteria [12] were followed throughout this study regarding patient selection, assays performance, and data analysis. Institutional board previously approved all practice and all participants signed informed consent terms. This study is in accordance with the ethical principles for medical research involving human subjects from the Declaration of Helsinki.

Clinicopathological data of cancer patients was collected from medical records and included age at diagnosis, TNM staging, tumor histological type, histological tumor grade, lymph nodal status, tumor size, and presence of distant metastasis.

2.2. Immunohistochemical Labeling for Nitrotyrosine (NT)

Nitrotyrosine (NT) is a residue formed by the action of peroxynitrite (derived from the reaction of nitric oxide and superoxide anion) on proteins. Paraffin-embedded sections were heated (30 min, 65°C), deparaffinized, and rehydrated. Sections were treated at room temperature with 2% bovine serum albumin and incubated overnight at 4°C with primary mouse anti-human antibodies against NT-labeled residues (diluted 1 : 300, Santa Cruz Biotechnology, clone sc-32757, USA), previously validated for human samples [13]. The secondary antibody, horseradish peroxidase, and 3,3′-diaminobenzidine (DAB) were provided by the commercial kit (Dako LSAB, Germany). In the last step, sections were weakly counterstained with Harry’s hematoxylin (Merck). For each case, negative controls were performed on serial sections by omitting the primary antibody incubation step. The intensity and localization of the immunoreactivity were examined with a photomicroscope (Leica DM 2500 and Leica DFC280, Leica, Germany).

2.3. Sample Processing for Determining the Tissue Oxidative Status

Frozen tissue samples were thawed, precisely weighted, and homogenized in sterile saline phosphate buffer 10 mM pH 7.4, at a final concentration of 100 mg tissue/mL. The mixture was centrifuged at 5000 ×g, 4°C during 10 minutes. Supernatants were collected and kept in ice bath until analysis. All described methods used this concentration of tissue homogenate, except when some specific dilution is highlighted. Heparinized blood samples were centrifuged at 1500 ×g, 4°C during 5 minutes. Plasma samples were separated for further analysis. All measurements were conducted at the same day of sample processing.

2.4. Measurement of Tissue Lipoperoxidation by High-Sensitivity Chemiluminescence

Lipoperoxidation of adjacent and tumoral tissue was evaluated as previously published, with some adaptations [14]. Aliquots of 250 μL of tissue homogenate (100 mg/mL) were added to 750 μL of saline phosphate buffer 10 mM pH 7.4, with addition of 10 μL of t-butyl 3 mM solution. For plasma analysis, 200 μL of sample was mixed with 780 μL of saline phosphate buffer 10 mM pH 7.4, with addition of 20 μL of t-butyl 3 mM solution. Readings were carried out in a Glomax luminometer (Glomax, Promega). The results were expressed as relative light units (RLU) and the entire curve profile was used as indicator of lipoperoxidation. The area under the curve (AUC) was obtained by area integration.

2.5. Determination of Lipid Hydroperoxide Level by the Ferrous Oxidation-Xylenol Orange (FOX) Method

Lipid hydroperoxide concentrations in samples were estimated by the FOX method as published by Victorino et al. [15]. Plasma or tissue homogenate aliquots of 50 μL were mixed with 50 μL of FOX reagent. Samples were incubated for 30 minutes in the dark at room temperature and the absorbance of the supernatant was measured at 550 nm and the results were expressed as μM hydroperoxide/mg tissue.

2.6. Carbonyl Content and Antimyeloperoxidase Determination

Carbonyl content was measured as estimate of oxidative injury in proteins [16]. Tissue homogenate or plasma aliquots of 200 μL were added in 2 tubes. Test tubes received 1 mL of dinitrophenylhydrazine (DNPH) 10 mM and blank tubes received 1 mL of HCL 2.5 M. Tubes were incubated during 1 hour in ice bath. After that, samples were successively incubated with 1.25 mL of trichloric acetic acid 20% and 10% in ice bath during 20 minutes each, with centrifugation between incubations (1400 ×g/15 minutes). Supernatants were discarded and pellets were twice treated with 1 mL of an ethanol/water solution (1 : 1). The final precipitates were dissolved in 1 mL of guanidine 6 M and were left for 24 hours at 37°C. Carbonyl content was calculated by obtaining the spectra at 355–390 nm of DNPH-treated samples, employing one blank tube for each test. The obtained peaks were employed to calculate carbonyl concentration using a molar extinction coefficient of 22 M⁻¹cm⁻¹. Results were expressed as nmol/mL/mg tissue. Myeloperoxidase was detected by a commercial ELISA kit following manufacturer’s instructions (IBL International, Germany), and the data were expressed as U anti-MPO/mL.

2.7. Total Radical-Trapping Antioxidant Parameter (TRAP)

TRAP was measured in pure breast tissue homogenates (100 mg/mL) or plasma samples (diluted 1 : 50). For TRAP calculation, the induction time of the sample (time for which the sample antioxidants can inhibit the ABAP action) was compared to that of the standard antioxidant (trolox) and expressed as μM trolox/g tissue [17].

2.8. Evaluation of Nitrite as Estimate of Nitric Oxide (NO) Levels

NO was estimated by measuring nitrite as previously described [18]. Homogenate or plasma samples (60 μL) were deproteinized, and the supernatants were recovered and incubated with cadmium granules. After 10 minutes, the Griess reagent (Sigma) was added to 200 μL of the supernatants, and the reactions were incubated for 10 minutes at room temperature. The absorbance was read at 550 nm using a standard microplate reader (Multiskan EX, LabSystems, Minnesota, USA). The final results were expressed as μM nitrite/mg tissue.

2.9. Estimation of MDA Levels by High-Performance Liquid Chromatography (HPLC)

MDA determinations were made using equipment HPLC-20AT Shimadzu equipped with a LC20AT pump and SPDM20A UV, diode array absorbance detector employing a C18 reverse phase column, as described by [15]. Aliquots of 160 μL of plasma samples, tissue homogenate, or standard solution reacted with 100 μL of 0.5 M perchloric acid. Samples were centrifuged for 5 minutes, 5000 ×g at 4°C. About 180 μL of supernatant was recovered to react with 100 μL of thiobarbituric acid for 30 minutes, at 95°C, and transferred to ice bath to stop reaction. 100 μL of 1 M NaH2PO4, pH 7.0, was added to stabilize sample pH. Further, samples were centrifuged for 10 minutes, 5000 ×g at 4°C. Mobile phase was composed of 65% 50 mM KH2PO4 buffer, pH 7.0, and 35% methanol HPLC grade. Readings were executed at 535 nm during 12 minutes with isocratic flow of 0.8 mL/minute and results were expressed as MDA peak height.

2.10. Homocysteine and TNF-α Levels

Homocysteine (Axis-Shield Diagnostics, Abbott Diagnostics Division, UK) and TNF-α levels (e-Bioscience, USA) were determined in aliquots of 200 μL of plasma or tissue homogenates by using commercial kits. Homocysteine was expressed as μmol/L and TNF-α as pg/mL.

2.11. Statistical Analysis

All analyses were conducted in triplicate sets. Statistical analysis was performed using GraphPad Prism 5.0, Microsoft Office Excel 2007, and OriginLab 7.5 software. Results were expressed as arithmetic means and errors of the means. Differences among groups were assessed by two-way analysis of variance (ANOVA) with post hoc Bonferroni’s test for the lipid peroxidation curves and by Student’s paired -test for the other parametric parameters. Nonparametric data was analyzed by Mann-Whitney or Wilcoxon matched-pairs tests. Correlations among parameters in plasma and tumoral tissue were also performed using Pearson or Spearman tests. All data were checked using the Grubbs test (GraphPad Quickcalcs) to eliminate significant outliers (). was considered statistically significant.

3. Results

Table 1 shows the clinicopathological characterization of the 50 patients enrolled in this study. The mean age at diagnosis was 53.8 years, ranging from 31 to 77 years. Most of tumors presented histological grade 2 and the mean tumor size was 2.9 cm. Regarding tumor subtype, a prevalence of luminal tumors was found (30% of patients presented luminal A tumors, 20% were triple negative, 26.6% had HER2 enriched, and 23.4% were typed as luminal B). Most women presented local or locoregional disease (TNM I/II, 83.3%; TNM III, 16.7%), without any presence of distant metastasis. None of the included women were overweight/obese at diagnosis. The number of patients did not allow dividing the groups regarding the molecular subtype.

Aiming at characterizing the redox status of adjacent and tumoral breast tissue samples, we performed the analysis of some markers of oxidative damage in lipids and proteins. Figure 1 shows the lipid peroxidation profile determined by high-sensitivity chemiluminescence. This method allows identifying the oxidative damage of RS on lipidic components located at the plasmatic membrane. As shown, the adjacent mammary tissue presented higher lipid peroxidation status than the tumoral tissue (). Other lipid peroxidation-derived metabolites did not vary (FOX and MDA levels, Figures 2(a) and 2(b)).

(a)

(b)

(a)

(b)

(c)

(d)

Elevated homocysteine levels (from μM/100 mg tissue in adjacent breast to μM/100 mg tissue in tumoral tissue, , Figure 2(c)) were found in the tumoral tissue when compared to the adjacent mammary breast. Antioxidant capacity of tumoral tissue was significantly higher than the adjacent breast ( nM trolox/g tissue in adjacent breast and nM trolox/g tissue in tumor, , Figure 2(d)).

Tumor samples displayed increased TNF-α levels ( pg/mL of homogenate in adjacent breast and pg/mL of homogenate in tumoral tissue, , Figure 3(a)) and NO ( μM/mg tissue in adjacent breast and μM/mg tissue in tumoral tissue, , Figure 3(b)).

(a)

(b)

The protein-induced oxidative modifications are represented in Figure 4. All tumor samples presented moderate/intense labeling for nitrotyrosine labeling, suggesting a prooxidant role for NO in breast cancer (Figure 4(a)). High carbonyl content (from nmol/100 mg tissue in adjacent breast to nmol/100 mg tissue in tumoral tissue, , Figure 4(b)) was found in breast tissue. Anti-MPO levels did not vary between groups ( U/100 mg tissue in adjacent breast and U/100 mg tissue in tumoral tissue, ). Semiquantitative analysis of nitrotyrosine (Figure 4(d)) showed augmented levels in TU samples when compared to the adjacent normal breast ( arbitrary unities in MA samples and arbitrary unities in TU samples, ).

(a)

(b)

(c)

(d)

We further performed Spearman analysis to investigate whether there was some correlation between the oxidative status of tumors and its respective plasma obtained from the same patient (Table 2). All parameters were compared. Significant positive correlations were found with plasmatic versus tumoral TNF-α (), tumoral nitrotyrosine versus plasmatic NO (), and plasmatic versus tumoral carbonyl contents ().

4. Discussion

It is known that oxidative stress is active during the carcinogenic process and correlates with disease prognosis in breast cancer patients [19, 20]. In spite of that, this is the first characterization of the oxidative status of human tumor samples in comparison with matched nontumoral adjacent mammary tissue. Our findings indicate that the breast tumor presents a variable oxidative profile. There was reduced oxidative stress as demonstrated by reduced lipid peroxidative reaction, revealed by the decrease of chemiluminescence and MDA levels and increased total antioxidant capacity (TRAP). Contrarily, nitrosative stress increased as nitrotyrosine labeling and NO was shown to be augmented in tumoral tissue with significant correlation between them.

Protein oxidation also was elevated in tumoral tissue possibly as a consequence of nitrosative stress. Our results showing high levels of TNF besides increased levels of NO and nitrotyrosine suggest a possible cross talk between nitrosative stress and inflammatory mediators in tumor tissue. This cross talk is enforced by the significant correlation between TNF-α, NO, nitrotyrosine, and the carbonyl content between tumor and its matched plasma sample. The mammary tissue presents a large content of adipocytes, which provides abundant feedstock for the occurrence of lipid peroxidation reactions. Polyunsaturated fatty acids that contain two or more double bonds are more susceptible to peroxidation [21]. Several RS may abstract the first hydrogen atom to produce a lipid peroxyl radical [22]. In this context, we first evaluated the lipid peroxidation chain by using a chemiluminescence-based analysis. Here, the initiation step is characterized by the ascending part of the curve, which is dependent on the antioxidant content of the tissue [23]. The analysis of this initial reaction revealed that the lipids from adjacent nontumoral tissue were more oxidized than the lipidic content of tumor samples. The occurrence of reduced lipid peroxidation in the breast cancer environment has been reported in nipple aspirate fluids, suggesting a role for the downregulation of lipid peroxidation products in carcinogenesis [24]. Low lipid peroxidation activates several redox signaling pathways that recruit antioxidant induction from the organism to the site of increasing RS production and this configures a survival adaptation [25, 26].

In association with the reduced lipid peroxidation profile of tumors, we further found unaltered levels of lipid peroxidation products in tumor samples, as hydroperoxides (FOX) and malondialdehyde (MDA), suggesting that other low molecular weight substances may affect the lipoperoxidative status of cells. These findings indicate that, in some instance, tumors are protected against lipid peroxidation, potentially by accumulating membrane and intracellular antioxidants that neutralize this process. This fact was corroborated by the enhanced antioxidant capacity detected in tumor samples when compared to normal adjacent tissue, which explains the reduced lipid peroxidation chain observed in breast tumors. Therefore, high antioxidant content inside breast tumors may be able to retard the initiation of lipid peroxidation process, which may have a regulatory role in cell adaptation to oxidative changes.

In spite of the enhanced antioxidant capacity of tumors, we found significant augmented protein carbonylation in the tumoral tissue (but not in the adjacent mammary breast). The carbonylation reaction is an irreversible posttranslational modification that occurred in protein structure that results from the reaction between amino acid residues with the low molecular weight aldehydes generated during the lipid peroxidation process [27–30] and it is reported as an oxidative marker locally produced in the cancerous breast [31].

We further detected increased homocysteine levels in breast tumors, suggesting the attack of thiol residues by RS originated in tumor microenvironment. Homocysteine regulates cell cycle, apoptosis, and oxidative stress responses [32]. A direct relationship between high homocysteine and enhanced carbonyl content has been demonstrated [33], indicating that the augmented carbonylation of tumor proteins can be induced by high homocysteine concentration.

In cancer cells, enhanced activity of proinflammatory cytokines leads to RS production [27]. A recent study of nipple aspirate fluids obtained from patients with breast cancer indicated that high levels of cytokines, as TNF-α, are concomitant with augmented protein carbonylation [34] and correlated with elevated systemic homocysteine [35], corroborating the present findings in tumor samples. Therefore, enhanced carbonyl content, homocysteine, and TNF-α level seem to comprise a network communicating with each other in the breast cancer microenvironment.

The prooxidative status found here in the tumoral tissue was probably sustained by its proinflammatory nature, as shown by TNF-α and NO levels in tumor samples. NO is a multifunctional molecule in cancer. Our data indicate a nitrosative function for this molecule inside breast tumor, as nitrotyrosine was found only in the tumor analysis and not detected in the nontumorous counterpart. In addition, the TNF-driven pathway is constitutively activated in breast cancer [8], inducing NO and increasing [36] and modulating oxidative stress in breast cancer cells [37]. Our previous publications have demonstrated that these patients carrying breast tumors present a variety of oxidative plasmatic modifications, and we have questioned if this fact could be related with tumor oxidative status. Therefore, we performed a correlation analysis aiming to understand the putative association between levels of oxidative stress parameters in plasma versus tumoral tissue. We have found significant correlations between plasmatic versus tumoral levels of TNF-α, NO/nitrotyrosine, and carbonyl content. Altogether, these data support that the systemic prooxidative status reported for several studies in breast cancer patients may be correlated with tumor-driven inflammation.

A recent study from our group [16] has demonstrated that the presence of the primary tumor mass is determinant for the sustained proinflammatory systemic status found in women with breast cancer, which included high NO, enhanced oxidative stress, and augmented TNF-α. Therefore, in spite of the reduced size of the tumor mass, it seems that the breast tumor microenvironment (cancer cells, infiltrated macrophages, and endothelial cells) is endowed with an enormous capability to promote profound modifications in the host organism, resulting in the persistent inflammatory status provoked here by TNF-α, NO, and RS production. This fact cannot be satisfactorily explained by the immune response against the tumor, since women presenting local breast disease have systemically established a Th2 immune status [11].

Another contributing factor to this redox scenario may be the components of tumor stroma. Tumor-associated fibroblasts can affect metabolically their adjacent cells, and cancer cells use the oxidative environment as advantage to obtain nutrients from the surrounding environment [38]. Further, sustained oxidative stress allows cancer-associated fibroblasts to become myofibroblasts, which secrete growth factors and cytokines [39] and yield high ROS generation [40]. This vicious cycle may also affect distant mammary cells by propagating the prooxidant signaling in a paracrine manner, which helps to explain the altered oxidative profile observed here in the distant mammary adjacent tissue.

In conclusion, this set of redox alterations found in breast tumors seems to be necessary to ensure the hallmarks of cancer biology, since RS have been implicated in oncogene activation, genomic instability, chemotherapy resistance, and the metastatic process [5]. Furthermore, it is known that enhanced antioxidant capacity has been strongly associated as an innate tumoral mechanism for acquiring chemoresistance [41]. The presented data point to the existence of a correlation between tumor proinflammatory mediators and their circulating levels, suggesting that the tumor may be a putative source that stimulates the onset of such substances in blood.

Conflict of Interests

Authors declare no conflict of interests.

Acknowledgments

The authors would like to thank Jesus Antônio Vargas for excellent technical assistance and CAPES, CNPq, and Fundação Araucária for providing financial support.

References

S. Ogura and T. Shimosawa, “Oxidative stress and organ damages,” Current Hypertension Reports, vol. 16, no. 8, article 452, 2014.
View at: Publisher Site | Google Scholar
A. R. Nourazarian, P. Kangari, and A. Salmaninejad, “Roles of oxidative stress in the development and progression of breast cancer,” Asian Pacific Journal of Cancer Prevention, vol. 15, no. 12, pp. 4745–4751, 2014.
View at: Publisher Site | Google Scholar
G. Landskron, M. De La Fuente, P. Thuwajit, C. Thuwajit, and M. A. Hermoso, “Chronic inflammation and cytokines in the tumor microenvironment,” Journal of Immunology Research, vol. 2014, Article ID 149185, 19 pages, 2014.
View at: Publisher Site | Google Scholar
B. Halliwell, “Oxidative stress and cancer: have we moved forward?” Biochemical Journal, vol. 401, no. 1, pp. 1–11, 2007.
View at: Publisher Site | Google Scholar
S. Toyokuni, K. Okamoto, J. Yodoi, and H. Hiai, “Persistent oxidative stress in cancer,” FEBS Letters, vol. 358, no. 1, pp. 1–3, 1995.
View at: Publisher Site | Google Scholar
P. K. Mahalingaiah and K. P. Singh, “Chronic oxidative stress increases growth and tumorigenic potential of MCF-7 breast cancer cells,” PLoS ONE, vol. 9, no. 1, Article ID e87371, 2014.
View at: Publisher Site | Google Scholar
D. C. Malins and R. Haimanot, “Major alterations in the nucleotide structure of DNA in cancer of the female breast,” Cancer Research, vol. 51, no. 19, pp. 5430–5432, 1991.
View at: Google Scholar
C. Yau and C. C. Benz, “Genes responsive to both oxidant stress and loss of estrogen receptor function identify a poor prognosis group of estrogen receptor positive primary breast cancers,” Breast Cancer Research, vol. 10, no. 4, article R61, 2008.
View at: Publisher Site | Google Scholar
V. J. Victorino, F. C. Campos, A. C. S. A. Herrera et al., “Overexpression of HER-2/neu protein attenuates the oxidative systemic profile in women diagnosed with breast cancer,” Tumor Biology, vol. 35, no. 4, pp. 3025–3034, 2014.
View at: Publisher Site | Google Scholar
A. C. S. A. Herrera, C. Panis, V. J. Victorino et al., “Molecular subtype is determinant on inflammatory status and immunological profile from invasive breast cancer patients,” Cancer Immunology, Immunotherapy, vol. 61, no. 11, pp. 2193–2201, 2012.
View at: Publisher Site | Google Scholar
C. Panis, V. J. Victorino, A. C. S. A. Herrera et al., “Differential oxidative status and immune characterization of the early and advanced stages of human breast cancer,” Breast Cancer Research and Treatment, vol. 133, no. 3, pp. 881–888, 2012.
View at: Publisher Site | Google Scholar
D. G. Altman, L. M. McShane, W. Sauerbrei, and S. E. Taube, “Reporting recommendations for tumor marker prognostic studies (REMARK): explanation and elaboration,” PLoS Medicine, vol. 9, no. 5, Article ID e1001216, 2012.
View at: Publisher Site | Google Scholar
R. Fernández-Durango, A. Fernández-Martínez, J. García-Feijoo et al., “Expression of nitrotyrosine and oxidative consequences in the trabecular meshwork of patients with primary open-angle glaucoma,” Investigative Ophthalmology and Visual Science, vol. 49, no. 6, pp. 2506–2511, 2008.
View at: Publisher Site | Google Scholar
C. Panis, A. C. S. A. Herrera, V. J. Victorino et al., “Oxidative stress and hematological profiles of advanced breast cancer patients subjected to paclitaxel or doxorubicin chemotherapy,” Breast Cancer Research and Treatment, vol. 133, no. 1, pp. 89–97, 2012.
View at: Publisher Site | Google Scholar
V. J. Victorino, C. Panis, F. C. Campos et al., “Decreased oxidant profile and increased antioxidant capacity in naturally postmenopausal women,” Age, vol. 35, no. 4, pp. 1411–1421, 2013.
View at: Publisher Site | Google Scholar
A. C. S. Herrera, V. J. Victorino, F. C. Campos et al., “Impact of tumor removal on the systemic oxidative profile of patients with breast cancer discloses lipid peroxidation at diagnosis as a putative marker of disease recurrence,” Clinical Breast Cancer, vol. 14, no. 6, pp. 451–459, 2014.
View at: Publisher Site | Google Scholar
L. G. Lemos, V. J. Victorino, A. C. Herrera et al., “Trastuzumab-based chemotherapy modulates systemic redox homeostasis in women with HER2-positive breast cancer,” International Immunopharmacology, vol. 27, no. 1, pp. 8–14, 2015.
View at: Publisher Site | Google Scholar
C. Panis, L. G. T. Lemos, V. J. Victorino et al., “Immunological effects of taxol and adryamicin in breast cancer patients,” Cancer Immunology, Immunotherapy, vol. 61, no. 4, pp. 481–488, 2012.
View at: Publisher Site | Google Scholar
F. Mannello, G. A. Tonti, A. Pederzoli, P. Simone, A. Smaniotto, and V. Medda, “Detection of superoxide dismutase-1 in nipple aspirate fluids: a reactive oxygen species-regulating enzyme in the breast cancer microenvironment,” Clinical Breast Cancer, vol. 10, no. 3, pp. 238–245, 2010.
View at: Publisher Site | Google Scholar
J. M. Hartikainen, M. Tengström, R. Winqvist et al., “KEAP1 genetic polymorphisms associate with breast cancer risk and survival outcomes,” Clinical Cancer Research, vol. 21, no. 7, pp. 1591–1601, 2015.
View at: Publisher Site | Google Scholar
E. Niki, “Lipid peroxidation: physiological levels and dual biological effects,” Free Radical Biology and Medicine, vol. 47, no. 5, pp. 469–484, 2009.
View at: Publisher Site | Google Scholar
A. Catalá, “Lipid peroxidation of membrane phospholipids generates hydroxy-alkenals and oxidized phospholipids active in physiological and/or pathological conditions,” Chemistry and Physics of Lipids, vol. 157, no. 1, pp. 1–11, 2009.
View at: Publisher Site | Google Scholar
A. N. C. Simão, A. A. Suzukawa, M. F. Casado, R. D. Oliveira, F. A. Guarnier, and R. Cecchini, “Genistein abrogates pre-hemolytic and oxidative stress damage induced by 2,2′-Azobis (Amidinopropane),” Life Sciences, vol. 78, no. 11, pp. 1202–1210, 2006.
View at: Publisher Site | Google Scholar
F. Mannello, G. A. M. Tonti, S. Pagliarani et al., “The 8-epimer of prostaglandin F2α, a marker of lipid peroxidation and oxidative stress, is decreased in the nipple aspirate fluid of women with breast cancer,” International Journal of Cancer, vol. 120, no. 9, pp. 1971–1976, 2007.
View at: Publisher Site | Google Scholar
K. S. Fritz and D. R. Petersen, “An overview of the chemistry and biology of reactive aldehydes,” Free Radical Biology and Medicine, vol. 59, pp. 85–91, 2013.
View at: Publisher Site | Google Scholar
G. Bauer, “Targeting extracellular ROS signaling of tumor cells,” Anticancer Research, vol. 34, no. 4, pp. 1467–1482, 2014.
View at: Google Scholar
O. O. Erejuwa, S. A. Sulaiman, and M. S. Ab Wahab, “Evidence in support of potential applications of lipid peroxidation products in cancer treatment,” Oxidative Medicine and Cellular Longevity, vol. 2013, Article ID 931251, 8 pages, 2013.
View at: Publisher Site | Google Scholar
C. Panis, “Unraveling oxidation-induced modifications in proteins by proteomics,” Advances in Protein Chemistry and Structural Biology, vol. 94, pp. 19–38, 2014.
View at: Publisher Site | Google Scholar
F. Guéraud, M. Atalay, N. Bresgen et al., “Chemistry and biochemistry of lipid peroxidation products,” Free Radical Research, vol. 44, no. 10, pp. 1098–1124, 2010.
View at: Publisher Site | Google Scholar
R. M. Domingues, P. Domingues, T. Melo, D. Pérez-Sala, A. Reis, and C. M. Spickett, “Lipoxidation adducts with peptides and proteins: deleterious modifications or signaling mechanisms?” Journal of Proteomics, vol. 92, pp. 110–131, 2013.
View at: Publisher Site | Google Scholar
F. Mannello, G. A. Tonti, and V. Medda, “Protein oxidation in breast microenvironment: nipple aspirate fluid collected from breast cancer women contains increased protein carbonyl concentration,” Cellular Oncology, vol. 31, no. 5, pp. 383–392, 2009.
View at: Publisher Site | Google Scholar
B. Olas, “Hydrogen sulfide in signaling pathways,” Clinica Chimica Acta, vol. 439, pp. 212–218, 2015.
View at: Publisher Site | Google Scholar
M. Sibrian-Vazquez, J. O. Escobedo, S. Lim, G. K. Samoei, and R. M. Strongin, “Homocystamides promote free-radical and oxidative damage to proteins,” Proceedings of the National Academy of Sciences of the United States of America, vol. 107, no. 2, pp. 551–554, 2010.
View at: Publisher Site | Google Scholar
F. Mannello, D. Ligi, and M. Canale, “Aluminium, carbonyls and cytokines in human nipple aspirate fluids: possible relationship between inflammation, oxidative stress and breast cancer microenvironment,” Journal of Inorganic Biochemistry, vol. 128, pp. 250–256, 2013.
View at: Publisher Site | Google Scholar
P. Ferroni, R. Palmirotta, F. Martini et al., “Determinants of homocysteine levels in colorectal and breast cancer patients,” Anticancer Research, vol. 29, no. 10, pp. 4131–4138, 2009.
View at: Google Scholar
S. Loibl, J. Bratengeier, V. Farines et al., “Investigations on the inducible and endothelial nitric oxide synthases in human breast cancer cell line MCF-7—estrogen has an influence on e-NOS, but not on i-NOS,” Pathology Research and Practice, vol. 202, no. 1, pp. 1–7, 2006.
View at: Publisher Site | Google Scholar
P. Mehlen, C. Kretz-Remy, J. Briolay, P. Fostan, M.-E. Mirault, and A.-P. Arrigo, “Intracellular reactive oxygen species as apparent modulators of heat-shock protein 27 (hsp27) structural organization and phosphorylation in basal and tumour necrosis factor α-treated T47D human carcinoma cells,” Biochemical Journal, vol. 312, part 2, pp. 367–375, 1995.
View at: Publisher Site | Google Scholar
U. E. Martinez-Outschoorn, S. Pavlides, A. Howell et al., “Stromal-epithelial metabolic coupling in cancer: integrating autophagy and metabolism in the tumor microenvironment,” International Journal of Biochemistry and Cell Biology, vol. 43, no. 7, pp. 1045–1051, 2011.
View at: Publisher Site | Google Scholar
A. Jezierska-Drutel, S. A. Rosenzweig, and C. A. Neumann, “Role of oxidative stress and the microenvironment in breast cancer development and progression,” in Advances in Cancer Research, vol. 119, chapter 3, pp. 107–125, Elsevier, 2013.
View at: Publisher Site | Google Scholar
U. Martinez-Outschoorn, F. Sotgia, and M. P. Lisanti, “Tumor microenvironment and metabolic synergy in breast cancers: critical importance of mitochondrial fuels and function,” Seminars in Oncology, vol. 41, no. 2, pp. 195–216, 2014.
View at: Publisher Site | Google Scholar
A. Mencalha, V. J. Victorino, R. Cecchini, and C. Panis, “Mapping oxidative changes in breast cancer: understanding the basic to reach the clinics,” Anticancer Research, vol. 34, no. 3, pp. 1127–1140, 2014.
View at: Google Scholar

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Copyright © 2016 C. Panis et al. This is an open access article distributed under the Creative Commons Attribution License, which permits unrestricted use, distribution, and reproduction in any medium, provided the original work is properly cited.

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