Reduced Basal Nitric Oxide Production Induces Precancerous Mammary Lesions via ERBB2 and TGFβ

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Abstract

One third of newly diagnosed breast cancers in the US are early-stage lesions. The etiological understanding and treatment of these lesions have become major clinical challenges. Because breast cancer risk factors are often linked to aberrant nitric oxide (NO) production, we hypothesized that abnormal NO levels might contribute to the formation of early-stage breast lesions. We recently reported that the basal level of NO in the normal breast epithelia plays crucial roles in tissue homeostasis, whereas its reduction contributes to the malignant phenotype of cancer cells. Here, we show that the basal level of NO in breast cells plummets during cancer progression due to reduction of the NO synthase cofactor, BH4, under oxidative stress. Importantly, pharmacological deprivation of NO in prepubertal to pubertal animals stiffens the extracellular matrix and induces precancerous lesions in the mammary tissues. These lesions overexpress a fibrogenic cytokine, TGFβ, and an oncogene, ERBB2, accompanied by the occurrence of senescence and stem cell-like phenotype. Consistently, normalization of NO levels in precancerous and cancerous breast cells downmodulates TGFβ and ERBB2 and ameliorates their proliferative phenotype. This study sheds new light on the etiological basis of precancerous breast lesions and their potential prevention by manipulating the basal NO level.

Introduction

One in eight women in the United States is diagnosed with breast cancer in their lifetime, making it the second leading cause of cancer death among women1. Of the 300,000 new breast cancer cases diagnosed in the US each year, nearly 30% are early-stage lesions including hyperplasia, atypia and in situ cancers1,2. Despite being precancerous, early-stage breast lesions are the precursor of invasive cancers, and over 40% of them could progress to invasive cancer if left untreated2. Because of the dramatic increase in the incidence as well as etiological and therapeutic uncertainties, early-stage breast lesions have become a major clinical challenge over the past decades2.

To understand the basis of early-stage breast lesions, a number of recent studies report the causative roles of different breast cancer risk factors, especially, those that are independent of genetic predisposition and can therefore be modified. These risk factors include a high-fat diet, moderate to heavy alcohol intake, smoking, low physical activity, diabetes, obesity and hypertension3,4,5,6,7,8,9. Interestingly, these different risk factors are commonly linked to aberrant production of nitric oxide (NO)10,11,12,13,14,15,16, a bioactive signaling molecule produced throughout the body. This led us to hypothesize that abnormal levels of NO in the breast might contribute to formation of precancerous breast lesions.

NO is produced by NO synthases 1–3 (NOS 1–3) using arginine as the substrate to exert pleiotropic functions. Its bioactivities can dramatically differ depending on the concentration, timing and context17,18,19,20. In canonical signaling, physiological stress promotes the production of large amounts of NO, particularly by the inducible NOS2, triggering proper functions of specialized cells including neurons, muscles, endothelia and immune cells21. Conversely, under the unstressed, normal physiological conditions, NO is produced at the basal steady-state level by the constitutive NOS1 (neuronal) and NOS3 (endothelial) in diverse cell types contributing to tissue morphogenesis, homeostasis and tissue-specific functions22,23,24,25. In mammary glands, NOS-1 and -3 are constitutively expressed and are elevated during pregnancy26,27,28, while NO production increases in the postpartum period29,30. This not only promotes alveolar (milk-producing unit) development, blood flow and nutrient uptake for milk production31,32, but also facilitates milk ejection27,33. Moreover, NO is secreted into the breast milk as an essential component for immunity and neonatal growth34.

In diseased states including cancer, however, NO production is often dysregulated. Some studies report that NO production increases during cancer progression18,35,36, while others report the opposite24,37,38. Thus, too much or too little NO might equally contribute to disease pathogenesis39,40. NO’s activities in cancer are also complex and contradictory41. NO can exert dichotomous effects on diverse cellular processes including proliferation, apoptosis, migration, invasion and angiogenesis. Such variations depend on NO’s concentration, context, timing, microenvironment, cancer type and stage18,20,41,42,43. For example, NO activates pro-tumoral signals (ERK and HIF1-α) at lower concentrations (<300 nM), but activates anti-tumoral signals (p53) at higher concentrations (>300 nM)42. Furthermore, NO could be produced by cancer cells or cancer-associated macrophages (M1 type), leading to either pro- or anti-tumoral effects41,44. This intricacy has led to conflicting reports and a notion that NO plays a double-edged role as both a cancer-promoter and -inhibitor17,18,20,45.

To make matters more complicated, in many diseases including cancer, NOS might be dysfunctional due to deprivation of the redox-sensitive cofactor, tetrahydrobiopterin (BH4), while being under oxidative stress. In this state, NOS fails to form the functional homodimer to produce NO and remains as monomers46. NOS monomers then produce superoxide instead of NO (“uncoupled”), exacerbating the disease pathogenesis47,48,49,50. Such alterations in the functionality of NOS might, at least in part, explain why NOS, in particular NOS2 isoform, is preferentially upregulated in many types of cancers51,52.

To support our hypothesis that aberrant NO production is involved in normal-to-precancerous progression of the breast epithelia, we have recently reported that non-malignant mammary epithelial cells (MECs) produce NO at the basal steady-state level upon interacting with the laminin-rich extracellular matrix (ECM)24,53. Such NO production is critical for the establishment of mammary tissue architecture and homeostasis24. On the other hand, in the malignant counterpart derived from the same patient, NO production is defective, contributing to formation of proliferative, disorganized structures in 3D ECM cultures24,53.

In the present study, we investigate whether aberrant NO production contributes to the formation of precancerous breast lesions from normal mammary epithelia using cell lines of a breast cancer progression series as well as animal models. Here, we show that the basal level of NO production in cultured MECs plummets along with cancer progression. This was primarily due to reduction of the NOS cofactor, BH4, under increased oxidative stress (NOS uncoupling), but was independent of NOS levels. Importantly, pharmacological deprivation of NO in developing mouse mammary glands led to the formation of multiple (peripheral) papillomas (precancerous mammary lesions)54,55,56,57,58 and desmoplastic ECM in all the animals tested. NO-deprived mammary glands exhibited overactivation of an oncogene, ERBB2, and a fibrogenic cytokine, TGFβ. These glands also highly expressed senescence markers, reported to be prevalent in precancerous lesions59,60,61. In addition, NO-deprived mammary glands displayed bi-lineage phenotype and stem cell-like properties, which are also reported to be prevalent in precancerous lesions62,63,64. Consistently, application of the BH4 precursor (sepiapterin) or a NO donor (SNAP or GSNO) to precancerous and cancerous breast cells normalized NO levels, suppressed TGFβ and ERBB2 signals and ameliorated proliferative phenotype. Our results unravel the critical contribution of deficient basal NO production to the pathogenesis of precancerous breast lesions.

Results

Basal level of NO production in cultured mammary epithelial cells plummets during normal-to-precancerous progression

We previously demonstrated that non-malignant MECs produce the basal steady-state level of NO immediately after contacting laminin, but not collagen, in the extracellular matrix (ECM)24. This observation is in agreement with a notion that NO production is largely influenced by chemical and mechanical properties of the tissue microenvironment such as the ECM53,65,66,67.

In our previuos studies, to test whether basal NO production is altered in breast cancer progression, we used the HMT-3522 breast cancer progression series composed of non-malignant S1 and malignant T4-2 cells68,69. S1 was derived from a benign mammary fibrocystic lesion and became spontaneously immortalized in culture68,70,71,72. S1 cells retain non-malignant characteristics, requiring EGF to grow in culture and being unable to form tumors in nude mice68,71,72. (The use of S1 cells is restricted to passages below 60 because of genotypic drift at higher passages71,72.) S1 cells were utilized to generate the malignant counterpart (HMT-3522-T4-2) by withdrawing EGF from the growth medium and serially transplanting cells into animals, without overexpressing oncogenes72,73. We showed that basal NO production in response to laminin is pronounced in non-malignant S1, but is impaired in malignant T4-2 cells24,53. This observation was confirmed using normal vs. malignant human breast tissues24.

In the present study, we attempted to test whether basal NO production is altered stepwise during malignant progression of MECs. We utilized the MCF10A breast cancer progression series, composed of four isogenic cell lines: MCF10A, AT1, DCIS.COM and CA1d74,75,76,77,78,79,80. MCF10A, harboring many characteristics of normal breast epithelium, was derived from a mammary fibrocystic lesion and was spontaneously immortalized in culture74. AT1, showing the features of atypical hyperplasia, was generated by transfecting mutant H-Ras into MCF10A cells and serially transplanting them into nude mice75,76. AT1 cells do not initially grow out as carcinomas in nude mice; however, within 2 years 25% of them become cancerous76. DCIS.COM, showing dysplastic comedo DCIS phenotype, was derived from cells of a hyperplastic lesion formed by AT1 cells in nude mice77. DCIS.COM cells do not initially grow out as carcinomas in nude mice; however, after 9 weeks half of them form tumors77. CA1d was derived from a tumor formed by AT1 cells after one year in animals78. 100% of CA1d cells form metastatic tumors in nude mice78.

We pulse-treated these cell lines with a drip of reconstituted laminin-rich ECM (lrECM, a.k.a. Matrigel) and determined the level of intracellular NO using a fluorescent probe DAF-FM24,81. While non-malignant (MCF10A) cells produced an appreciable level of DAF FM signal, the level was dramatically (~−60%) reduced in precancerous (AT1) cell and remained low in cells with more advanced stages (DCIS and CA1d) (Fig. 1A). As a complementary approach, we measured the level of the NO metabolite (nitrite) in the conditioned media of cells cultured in 3D lrECM using a fluorescent probe DAN24,82 and observed similar results (Fig. 1B). Furthermore, we analyzed the level of S-nitrosocysteine (SNOC, a NO-dependent protein modification) as an indicator of NO production. Consistently, the cytosolic, but not nuclear, SNOC level progressively declined along with cancer progression (Fig. 1C).

Figure 1
figure1

Non-malignant mammary epithelial cells produce the basal level of nitric oxide (NO) in 3D ECM cultures, whereas the level plummets along with breast cancer progression. (A) (Left) Cell lines of MCF10A breast cancer progression series (10A; non-malignant; AT1: premalignant; DCIS: ductal carcinoma in situ; and CA1d: malignant)74,75,76,77,78,79,80 cultured with 5% Matrigel drip and stained with the fluorescent NO probe DAF-FM DA. (Right) Quantification of DAF-FM DA signal/cell in the series. (See DAF-FM DA signals of a panel of normal vs. cancerous MECs in Supplementary Fig. 1A,B). (B) The level of NO metabolite nitrite in the conditioned media of the progression series. (C) (Left) Cell lines of the progression series stained with an antibody against S-nitrosocysteine (S-NOC). (Right) Quantification of S-NOC level in the nucleus (N) vs. cytosol (C) of the series. AU: arbitrary unit. Error bars: mean ± STDEV. *p < 0.05; **p < 0.01; and ***p < 0.001.

To test the generality of this phenomenon, we compared basal NO production in response to lrECM among a panel of normal/non-malignant vs. cancerous breast cell lines using the NO probe DAF-FM. The specificity of the signal was confirmed by quenching it with the NOS inhibitor, L-NAME (2.5 mM), an L-arginine analog that competitively inhibits the substrate binding to NOS (IC50 ~ 70 μM)83 [and to arginase (IC50 ~ 27 mM)84,85]. DAF-FM signals were generally much higher in normal/non-malignant MECs than breast cancer cells (Supplementary Fig. 1A,B), consistent with previous reports24,53,86. These results altogether demonstrate that the levels of basal NO become lower in MECs along with cancer progression.

NOS-1 and -3 levels remain high, while NOS-2 level remains low, in all cell lines of the breast cancer progression series

NO is produced by three isoforms of NO synthases (NOS 1–3)21. To determine which isoform is involved in NO production in MECs, we examined the level of each NOS isoform in the MCF10A progression series. In non-malignant MCF10A cells, NOS-1 and -3 were both expressed at high levels, whereas NOS-2 was undetectable (Fig. 2A). We then examined the level of each NOS isoform in normal mouse mammary glands. The expression patterns of NOS isoforms were the same as those in MCF10A, consistent with previous reports (Fig. 2B)26,27,28. Interestingly, throughout the entire progression series, NOS expression patterns did not change. NOS-1 and -3 remained high, while NOS-2 remained low (Fig. 2A). This result suggests that NOS levels have no relevance to reduction of basal NO level in cell lines of breast cancer progression series.

Figure 2
figure2

Nitric oxide synthase (NOS)-1 and -3 are involvd in production of basal NO in MECs. (A) (Top) NOS-1, -2 or -3 staining of the MCF10A breast cancer progression series. Scale bars: 20 μm. (Bottom) Quantification of NOS signal/cell. AU: Arbitrary unit. (B) (Left) NOS-1, -2 or -3 staining of mouse mammary glands (10 weeks old, virgin female). Nuclei were counterstained with DAPI (blue). Scale bars: 50 μm. (Right) Quantification of NOS signal/cell. (C) (Left) S-NOC staining of MCF10A cells expressing scramble, NOS-1, -2 or -3 shRNA. Nuclei were counterstained with DAPI (blue). Scale bars: 20 μm. (Right) Quantification of SNOC signal/cell. (D) S-NOC staining of MCF10A cells with double knockdown (KD) of NOS-1 and -3 using different combinations of shRNA and siRNA. (Top 2 rows, left) S-NOC staining of MCF10A cells expressing scramble, NOS-2 or -1 shRNA, which were further transfected with NOS-3 siRNA. (Top right) Quantification of S-NOC signal/cell. (Bottom 2 rows, left) S-NOC staining of MCF10A cells expressing scramble, NOS-2 or -3 shRNA, which were further transfected with a NOS-1 siRNA. (Bottom right) Quantification of S-NOC signal/cell. Note that while KD of NOS-1 or -3 alone partially inhibited SNO, double KD of NOS-1/NOS-3 abrogated SNOC. Scale bars: 50 μm.

Basal level of NO production in mammary epithelial cells is mediated by NOS-1 and -3

To confirm that NOS-1 and -3 are indeed involved in basal NO production in MECs, we nearly depleted each isoform with a specific shRNA in non-malignant MCF10A cells (Supplementary Fig. 2A), which were shown to produce the highest level of NO among all cell lines of the progression series (Fig. 1A). We then examined which NOS depletion had impaired NO production by comparing SNOC levels. Single knock-down (KD) of either neuronal NOS1 or endothelial NOS3 partially reduced SNOC level, whereas KD of inducible NOS2 had no effect (Fig. 2C). Conversely, simultaneous inhibition of NOS3 in NOS1-KD cells or NOS1 in NOS3-KD cells with a specific siRNA (Fig. 2D) or with a small molecule inhibitor (Supplementary Fig. 2B) almost abrogated SNOC signal. These results suggest that NOS-1 and -3 (but not NOS-2) equally participate in production of the basal level of NO in MECs.

Reduced NO production in cell lines of breast cancer progression series correlates with increased acidity and oxidative stress that depletes the NOS cofactor BH4

We further examined why NO production dramatically declines in cell lines of the breast cancer progression series, while NOS levels remain unchanged (Figs 1A, 2A). We postulated that this might be attributed to certain physiological traits associated with cancer progression that could debilitate NOS functions. To test this, we measured the intracellular pH and oxidative stress (superoxide and total reactive oxygen species). Acidification and oxidative stress are hallmarks of cancer metabolism87 and also known to attenuate NOS functions49,88,89,90. As expected, the acidity and oxidative stress were significantly elevated along with cancer progression (Fig. 2A–C).

In particular, oxidative stress has been shown to deplete the essential NOS cofactor, BH4. BH4 helps tether two NOS monomers to form the functional NOS homodimer, allowing for coupling two reactions required for NO production: (1) reduction of molecular oxygen and (2) oxidation of arginine91. When BH4 (or arginine) is deficient, however, NOS remains as monomers, and these two reactions are uncoupled, releasing superoxide (from the former reaction only) instead of producing NO —a phenomenon termed ‘NOS uncoupling’49,88.

To test this possibility, we measured the intracellular BH4 level in cell lines of the breast cancer progression series. As expected, BH4 level was dramatically (~−40%) reduced in normal-to-precancerous transition and remained low thereafter (Fig. 2D). This paralleled the dramatic increase of superoxide levels, suggesting the possible occurrence of NOS uncoupling (Fig. 2B). We additionally tested for the potential involvement of known endogenous NOS inhibitors, asymmetric dimethylarginine (ADMA) and dynein light chain LC8-Type 1 (DYNLL1)92, in reduction of NO level in the progression series. ADMA and DYNLL1 levels did not significantly change throughout the progression series (except for some increase of ADMA in DCIS) (Fig. 3E, Supplementary Fig. 3), excluding their major contributions. These results altogether strongly suggest that deficiency of the NOS cofactor, BH4, is a critical contributor to reduction of basal NO producion in MECs during cancer progression.

Figure 3
figure3

Decrease of the basal NO level along with breast cancer progression parallels the dramatic increase in acidity and oxidative stress and the decline of the NOS cofactor BH4. (A) Cells of the MCF10A progression series stained with pH probe. (Left) Cells treated with pH standard (pH 5.5–7.5) are shown on the right, whereas the analytes are shown on the left. Scale bars: 100 μm. (Right) pH level of the series. Error bars: mean ± STDEV. ***p < 0.001. (B) (Left) Cells of the MCF10A progression series stained with superoxide probe. Scale bars: 20 μm. (Right) Quantification of superoxide signal/cell. (C) Total level of reactive oxygen species in the MCF10A progression series. (D) BH4 level of the MCF10A progression series. Error bars: mean ± STDEV. ***p < 0.001. (E) Images of western blots against endogenous NOS inhibitors, ADMA and DYNLL1, for cell lines of the MCF10A progression series. β-actin serves as the loading control. (See the raw gel image in Supplementary Fig. 3).

Pharmacological deprivation of NO impairs mouse mammary gland development, but induces desmoplastic ECM due to overactivation of TGFβ

To determine whether reduction of NO level contributes to breast cancer pathogenesis in vivo, we pharmacologically inhibited NO production in inbred wild-type mice (BALB/c) for a duration of 6 weeks (from 4 to 10 weeks old) by intraperitoneal (i.p.) injection of L-NAME (NOS antagonist, 20 mg/kg), in comparison to control (vehicle) and L-arginine (NOS substrate [agonist], 20 mg/kg) treatments. L-NAME-treated mouse mammary glands completely lacked alveoli, demonstrating the clear developmental defect, consistent with NO’s critical roles in mammary gland development (Fig. 4A)27,29,31,32,33,34. To confirm altered NO levels, drug-treated mammary glands were stained for SNOC. Control glands exhibited the basal level of SNOC, whereas L-arginine-treated glands showed dramatically elevated SNOC level. On the other hand, L-NAME-treated glands exhibited almost undetectable SNOC level (Fig. 4B, Supplementary Fig. 4A).

Figure 4
figure4

Deprivation of NO in developing mouse mammary glands stiffens the ECM and induces precancerous lesions, accompanied by upregulation of TGFβ and ERBB2 and induction of senescence. (A) Whole mounts of carmine-stained 4th mammary glands of mice after i.p. treatment with control (PBS), L-arginine or L-NAME for 6 weeks (from 4 weeks to 10 weeks old). Scale bars: top, 10 mm; bottom, 200 μm. (B) Representative images of S-NOC staining (top), SHG (collagen) (second row) and phospho-SMAD3 (TGFβ signal) staining (bottom 2 rows) of drug-treated mammary glands. Nuclei were counterstained with DAPI (blue). Scale bars: 50 μm. (See the original micrographs and quantification of S-SNOC, SHG and phospho-SMAD3 levels in Supplementary Fig. 4A–C). (C) H&E staining of drug-treated mammary glands. Note that intraductal papillomas are indicated with pink asterisks (*). Scale bars: 50 μm. (D) Representative images of staining for ERBB2 (top), HP1 (second row), β-Gal (third row), p21 (fourth row) and p27 (bottom row) of drug-treated mammary glands. Nuclei were counterstained with DAPI (blue). Scale bars: 50 μm (See the quantification of ERBB2, HP1, β-Gal, p21 and p27 staining in Supplementary Fig. 4D–H).

Reduced NO bioavailability in patients with chronic conditions, such as diabetes, cardiovascular disease and obesity, often leads to formation of stiff, desmoplastic (fibrotic) ECM which is directly linked to increased cancer risk93,94,95. To test this possibility, we measured the density of collagen fibers in drug-treated mammary tissues using second harmonic generation (SHG) technique96. As expected, periductal collagen level was dramatically elevated in L-NAME-treated mammary tissues, compared to control or L-arginine-treated tissues (Fig. 4B, Supplementary Fig. 4B). To determine the cause of the desmoplastic ECM in L-NAME-treated mammary tissues, we tested for the involvement of transforming growth factor β (TGFβ), the major activator of collagen biosynthesis97. We stained mammary tissues for phospho-SMAD3 (active form), the downstream effector of TGFβ signaling. Phospho-SMAD3 level, in fact, was dramatically (>5-fold) elevated in L-NAME-treated mammary glands (Fig. 4B, Supplementary Fig. 4C), suggesting strong activation of TGFβ signals upon NO depletion. These results demonstrate that NO deprivation in mammary glands of prepubertal to pubertal mice impairs gland development, but induces desmoplastic ECM along with overactivation of TGFβ signaling.

NO-deprived mouse mammary glands form precancerous lesions that overexpress ERBB2

Formation of desmoplastic ECM indicates the occurrence of certain pathological conditions in NO-deprived mammary tissues95. Histological examination strikingly revealed that every L-NAME-treated animal (n = 6) formed multiple (peripheral) papillomas —precancerous mammary lesions54,55,56,57,58 —visualized by H&E staining of serial sections. In contrast, neither control nor L-arginine-treated animals formed such lesions (Fig. 4C). We then tested for the possible involvement of the ERBB2 oncogene, highly linked to precancerous progression of MECs98,99,100,101. While a change in the ERBB2 gene locus is found in 20~30% cases of invasive breast cancers, it is even more prevalent in premalignant breast lesions (~50%), suggesting that a change in ERBB2 gene is an early event in breast carcinogenesis102,103,104. As expected, ERBB2 levels were dramatically (>3-fold) elevated in L-NAME-treated mammary glands (Fig. 4D, Supplementary Fig. 4D). It is reported that overexpression of ERBB2 in normal or cancerous breast cells induces cellular senescence as an anti-carcinogenic mechanism105,106,107. In addition, senescence is shown to be the most prevalent in precancerous lesions, compared to normal or invasive lesions59,60,61. Therefore, to test whether the L-NAME-treated glands had undergone senescence, we determined the levels of well-established senescence markers: heterochromatin protein 1 (HP1), β-Galactosidase (β-Gal), p21 and p2760,61,108. All these senescence markers were highly elevated in L-NAME-treated glands, whereas they were almost undetectable in control or L-arginine-treated glands (Fig. 4D, Supplementary Fig. 2E–H). These results demonstrate that NO deprivation in mouse mammary glands induces precancerous lesions that strongly express ERBB2, accompanied by the occurrence of senescence.

Inhibition of NO in non-malignant human mammary epithelial cells in 3D ECM cultures impairs acinar morphogenesis and upregulates TGFβ and ERBB2

To determine whether the effects of NO modulation on mouse mammary glands were intrinsic to MECs or due to stromal and systemic influence, we treated mono-cultures of non-malignant human MECs (MCF10A cells) with L-NAME, in comparison to control (PBS) or L-arginine, in 3D lrECM for 3 weeks. Consistent with our previous report24, L-NAME impaired formation of mammary acini, but induced formation of disorganized, proliferative aggregates (Fig. 5A, Supplementary Fig. 5A). These colonies showed aberrant apico-basal polarity, indicated by mislocalization of the basal marker (integrin α6) and apical marker (GM130), as well as the loss of lumens (demarcated by cleaved caspase 3) (Fig. 5A, Supplementary Fig. 5B)24. L-NAME dramatically elevated phospho-SMAD3 and ERBB2, as well as senescence markers, p21 and β-Gal in MECs in 3D lrECM cultures (Fig. 5B, Supplementary Fig. 5C)109, consistent with the above in vivo results (Fig. 4B,D).

Figure 5
figure5

Deprivation of NO in non-malignant mammary epithelial cells in 3D cultures induces disorganized colonies, accompanied by induction of TGFβ, ERBB2 and senescence markers. (A) Representative images of MCF10A cells cultivated in 3D ECM under treatment of control (PBS), L-arginine or L-NAME for 3 weeks. Top 2 rows: phase images. Middle 3 rows: staining for the basal marker, integrin α6 (ITGA6) or apical marker, GM130. Bottom 2 rows: staining for lumen marker, cleaved caspase 3 (CC-3). Nuclei were counterstained with DAPI (blue). Scale bars: 20 μm. (See the quantification of colony size, and plot profiles of ITGA6, GM130 and CC-3 signals in Supplementary Fig. 5A,B). (B) Representative images of phospho-SMAD3 (top 2 rows), ERBB2 (rows 3–4), p21 (rows 5–6) or β-Gal (bottom 2 rows) staining of drug-treated MCF10A cells in 3D cultures. Nuclei were counterstained with DAPI (blue). Scale bars: 20 μm. (See the quantification in Supplementary Fig. 5C).

To determine the generality of the effects of modulating NO level, we applied L-arginine or L-NAME to ERBB2-positive (amplified) SKBR3 breast cancer cells110. Surprisingly, even after a short-term (overnight) treatment, L-NAME dramatically (>3-fold) elevated the level and membrane-localization of ERBB2 over control, whereas L-arginine almost abrogated them (Supplementary Fig. 5D). These results suggest that the effects of NO modulation on mammary glands we observed are largely intrinsic to MECs and might have manifested soon after treatment.

Inhibition of NO in breast epithelial cells induces bi-lineage and stem cell-like phenotype in both mammary glands and 3D ECM cultures

It has been reported that activation of certain oncogenic pathways, such as ERBB2, in normal or cancerous MECs could induce stem cell-like properties101,111. These cells are characterized by luminal (CK8/18)/basal (CK14) bi-lineage phenotype, as well as high expression of stem cell markers such as CD44, and are also found to be prevalent in precancerous lesions62,63,64.

Since NO deprivation dramatically elevated ERBB2 in wild-type mouse mammary glands (Fig. 4D, Supplementary Fig. 4D), we tested whether this might have induced stem cell-like properties101. First we tested for the occurrence of bi-lineage phenotype by co-staining drug-treated mammary glands for CK8/18 (luminal) and CK14 (basal)62. As previously reported, control and L-arginine-treated mammary glands showed mutually exclusive pattern of CK8/18 vs. CK14112. In contrast, L-NAME-treated glands showed a significant (>10-fold) increase in CK18high/CK14high bi-lineage cells (Fig. 6A, Supplementary Fig. 6A)62.

Figure 6
figure6

Deprivation of NO induces bi-lineage phenotype and expression of stem cell markers in mammary epithelial cells both in vivo and in 3D cultures. (A) CK14 (basal) and CK8/18 (luminal) staining of mouse mammary glands treated with control (PBS), L-arginine or L-NAME for 6 weeks. Co-localization of CK14 and CK8/18 was captured with ImageJ. Scale bars: 100 μm. (See the quantification in Supplementary Fig. 6A). (B) Representative images of drug-treated mammary glands stained for stem cell markers: alkaline phosphatase (AP) (top 2 rows), CD44 (middle 2 rows) or CD24 (bottom 2 rows). Nuclei were counterstained with DAPI (blue). Scale bars: 50 μm. (See the quantification in Supplementary Fig. 6B–D). (C) CK14 and CK8/18 staining of non-malignant MCF10A cells cultivated in 3D ECM in the presence of control (PBS), L-arginine or L-NAME for 3 weeks. Scale bars: 50 μm. (See the quantification in Supplementary Fig. 6E). (D) Drug-treated MCF10A cells in 3D cultures stained for AP (top 2 rows), CD44 (middle 2 rows) or CD24 (bottom 2 rows). Nuclei were counterstained with DAPI (blue). Scale bars: 50 μm. (See the quantification in Supplementary Fig. 6F–H).

Next, we tested for the induction of stemness by staining the drug-treated mammary glands for stem cell markers, alkaline phosphatase (AP, a pluripotent stem cell marker)113, CD44 (another stem/progenitor marker) and CD24 (the luminal lineage marker)114,115,116. In both humans and mice, CD44high/CD24low phenotype is the predominant marker for multipotent stem/progenitor cells that have the highest repopulating (i.e., tumor-initiating) potential, while CD44high/CD24high and CD44low/CD24high phenotypes are the markers for cells “committed” to luminal differentiationin114,115,116,117. (CD44high/CD24high phenotype, nevertheless, is linked to increased drug-resistance118). In control and L-arginine-treated glands, the three stem cell markers, AP, CD44 and CD24, were virtually all absent. In contrast, in L-NAME-treated mammary glands, both AP and CD44 were strongly expressed in all the epithelia, whereas CD24 was mostly expressed in the luminal layer and expressed at low to moderate levels in the basal layer. (Fig. 6B. Supplementary Fig. 6B–D). These results demonstrate that L-NAME-treatment of mammary glands induces the stem cell population (CD44high/CD24low) on the basal layer, as well as another population of cells committed to luminal differentiation (CD44high/CD24high) on the luminal layer117.

We tested whether this in vivo phenotype could be recapitulated in mono-cultures of human MECs in 3D lrECM. Similar to our in vivo results, 3D colonies of control and L-arginine-treated non-malignant MCF10A cells showed distinct bi-layers of CK8/18-positive (luminal) vs. CK14-positive (basal) cells (Only 5~7% of cells were CK18high/CK14high bi-lineage). In contrast, L-NAME-treated cells were virtually all (>70%) CK18high/CK14high bi-lineage (Fig. 6C, Supplementary Fig. 6E). Stem cell markers, AP, CD44 and CD24, were almost undetectable in control and L-arginine-treated colonies. Conversely, in L-NAME-treated colonies, the expression of AP and CD44 was strongly positive throughout; CD24 expression was highly elevated on the periphery, but remained low in the center (marking the peripheral cells as CD44high/CD24high vs. central cells as CD44high/CD24low) (Fig. 6, Supplementary Fig. 6F–H). These results altogether demonstrate that L-NAME-treatment of normal/non-malignant MECs of humans and mice, both in culture and in vivo, respectively, induces a stem cell-like population with CK18high/CK14high bi-lineage phenotype and CD44high/CD24low expression.

Inhibition of NO in breast epithelial cells promotes formation of mammospheres enriched for stem cell-like cells

To further validate the induction of stemness by L-NAME treatment, drug-treated MCF10A cells were cultivated on PolyHEMA-coated (non-adherent) plates, which allows for detection of self-renewal capacity through formation of mammospheres119,120,121,122,123,124. For mammosphere formation assay as described previously119,120,123,124, cells were seeded at the densities of 1,250~10,000 cells/48-well. Both L-NAME and L-arginine-treatments increased the size, number and formation efficiency of mammospheres over control; however, L-NAME yielded the values twice as much as L-arginine (Fig. 7A–D, Supplementary Fig. 7A). The proportions of CK18high/CK14high bi-lineage cells within mammospheres were significantly (>4-fold) higher in L-NAME and L-arginine-treated spheroids than control spheroids (Fig. 7E, Supplementary Fig. 7B), attesting to the increase of stem cell-like populations62,112,125.

Figure 7
figure7

Deprivation of NO elevates self-renewal potential of non-malignant mammary epithelial cells. (A) Representative images of mammospheres derived from MCF10A cells grown on PolyHEMA-coated plates under the treatment of control (PBS), L-arginine or L-NAME for one week. Scale bars: 200 μm (top 2 rows) and 50 μm (bottom row). (B) The size of mammospheres derived from drug-treated MCF10A cells. (C) The number of spheroids formed at each seeding number. (See the micrographs of spheroids in Supplementary Fig. 7A). (D) Mammosphere forming efficiency at each seeding number. Mammosphere forming efficiency (%) = (# of spheroids)/(# of cells seeded) × 100119,120. Statistical significance between different treatments was determined by two-way ANOVA analysis with Bonferroni post hoc test175. Error bars: mean ± STDEV. **p < 0.01; ***p < 0.001. (E) Staining of mammospheres for the basal marker, CK14, and luminal marker, CK8/18. Co-localization of CK14 and CK8/18 was captured with ImageJ. (See the quantification in Supplementary Fig. 7B). (F) Limiting dilution analysis to determine the sphere forming frequency at clonal densities (≥200 cells/96-well)126. (Top) The graph plotted with the Y-axis as Ln (fraction of negative wells) and X-axis as seeding number. (Bottom) The sphere forming frequency corresponding to −(slope) of the line of best fit. (G) Staining of paraffin-embedded/sectioned mammospheres129 for stem cell markers CD44 and CD24. Scale bars: 20 μm (see the quantification of CD44 and CD24 levels in Supplementary Fig. 7C,D). (H) FACS analysis to determine the expression of CD44 and CD24 in cells dissociated from mammospheres. Isotype controls were used to set threshold gate.

Aiming to differentiate the effects of L-NAME from those of L-arginine, we performed a limiting dilution assay on drug-treated MCF10A cells that determines the abundance of cells capable of forming spheroids at clonal densities (200~1600/96-well)126,127. L-NAME treatment elevated the abundance of spheroid-forming cells by 5-fold over control and 8-fold over L-arginine treatment (Fig. 7F). These results altogether demonstrate that L-NAME treatment greatly increased the abundance of stem cell-like cells that possess clonal expansion capacity.

To further confirm the stemness of drug-treated spheroids, we measured the levels of stem cell markers, CD44 and CD24128, by immunofluorescence imaging of paraffin-embedded/sectioned spheres129. L-NAME-treated spheroids were strongly positive for CD44, whereas L-arginine-treated spheroids showed little or no expression. CD24 expression, on the other hand, was low in all conditions (Fig. 7G, Supplementary Fig. 7C,D).

As a complementary approach, we performed FACS analysis on cells dissociated from mammospheres. Consistent with the result from immunofluorescence imaging, L-NAME-treated mammospheres showed a dramatic increase in CD44 level. About 50% of cells were CD44 positive, and 1/4 of these CD44-positive cells (11.5% of the total cells) were CD44high/CD24low, cells with the highest repopulating potential114,115,116,117 (Fig. 7H). On the other hand, there were almost no (0.2~0.6%) CD44-positive cells in control and L-arginine-treated mammospheres. While CD24 level increased in L-arginine-treated (+6.5%) and L-NAME-treated spheroids (+24.1%), a significant fraction of cells (46~65%) showed low expression levels (Fig. 7H). These results altogether demonstrate that L-NAME-treatment elevated stem cell-like cells (CD44high/CD24low) which have the highest self-renewal ability and clonogenicity128.

Normalization of NO levels with the BH4 precursor, sepiapterin, ameliorates the malignant phenotype of breast cancer cells

To further test whether dysregulated NO levels contribute to the phenotype associated with breast cancer progression, we sought to normalize NO levels in precancerous and cancerous MECs. We showed above that reduced basal NO production in cultured MECs along with cancer progression was linked to oxidative depletion of the NOS cofactor, BH4, which triggers NOS uncoupling (Figs 1A–C, 2B–D)49,88. In an attempt to ameliorate the conditions of diseases including breast cancer, the BH4 precursor, sepiapterin, has been successfully utilized for ‘recoupling’ NOS in a number of cell culture and preclinical studies49,130,131,132,133,134.

We tested whether the application of sepiapterin could help normalize NO levels in precancerous and cancerous MECs in 3D lrECM cultures and whether this could ameliorate the malignant phenotype. After cultivation of the MCF10A progression series in the presence of sepiapterin at 20 μM49, NO levels of precancerous and cancerous cell lines (AT1, DCIS and CA1d) were restored to the levels comparable to (or at least half of) the level of non-malignant MCF10A cells. In contrast, NO level in non-malignant MCF10A cells did not change after sepiapterin treatment (Fig. 8A). Importantly, 20 μM of sepiapterin dramatically (>50%) reduced proliferation indices (i.e., colony size and Ki67 positivity) of precancerous and cancerous cell lines, but not of non-malignant cells (Fig. 8B). This was accompanied by a dramatic reduction in the levels of phospho-SMAD3 and ERBB2, which otherwise were pronounced in precancerous and cancerous cells (Fig. 8C). These results confirm that deficiency of BH4 is a major contributor to reduced basal NO production and malignant phenotype of precancerous and cancerous MECs.

Figure 8
figure8

BH4 precursor, sepiapterin, normalizes NO level and ameliorates malignant phenotype of precancerous and cancerous cells. (A) (Top) Cell lines of the MCF10A progression series cultured in 5% Matrigel drip with or without sepiapterin (20 μM) and stained with the NO probe DAF-FM DA, Scale bars: 50 μm. (Bottom) Quantification of DAF-FM signal/cell. AU: Arbitrary unit. (B) (Left top) Representative images of the MCF10A progression series cultivated in 3D ECM with or without sepiapterin (20 μM). (Left bottom) Quantification of colony size. (Middle top) Cell lines in the series cultivated in 3D ECM with or without sepiapterin (20 μM) and stained for Ki67. Scale bars: 50 μm. (Right top) Nuclei were counterstained with DAPI (blue) and merged with Ki67. Scale bars: 50 μm. (Right bottom) Percent of Ki67-positive cells/colony. (C) (Top) Representative images of the progression series cultivated in 3D ECM with or without sepiapterin (20 μM) and stained for phospho-SMAD3 or ERBB2. Nuclei were counterstained with DAPI (blue). Scale bars: 20 μm. (Bottom) Quantification of phospho-SMAD3 (left) and ERBB2 levels (right) of the progression series. Error bars: mean ± STDEV. *p < 0.05; **p < 0.01 and ***p < 0.001. Note that the effects of sepiapterin are only discernible in precancerous and cancerous cells, but not in non-malignant cells. (See the results of different concentrations of sepiapterin in Supplementary Fig. 8). (D) Mammary tumors from MMTV-PyMT mice (18 weeks, n = 4) were ex vivo 3D cultured with vehicle (PBS), L-NAME (2.5 mM, NOS inhibitor) or sepiapterin (100 µM) for 1 week. First raw: normal mouse mammary glands. Left column: 100x; right column: 400x H&E images of the boxed areas of the images in left column. Arrow heads: vessels. Scale bars: 50 µm. Note the restoration of normal-like glands after sepiapterin treatment vs. worsened proliferative phenotype after L-NAME treatment. Also, note the significant increase in the vasculature after sepiapterin treatment.

To test whether these effects of sepiapterin are dose-dependent, we treated the MCF10A progression series cultivated in 3D lrECM with a different concentration of sepiapterin (0, 20 or 100 μM). The increasing concentrations of sepiapterin (20 to 100 μM) progressively normalized NO levels in precancerous and cancerous cells, without affecting that of MCF10A cells (Supplementary Fig. 8A). Nevertheless, the growth-suppressive effects (by colony size and Ki67 positivity) of sepiapterin did not differ between the concentrations of 20 and 100 μM (Supplementary Fig. 8B–D). This suggests that the activity of sepiapterin is threshold-dependent, rather than concentration-dependent, at least within this range.

Furthermore, sepiapterin (20 and 100 μM) helped “normalize” the cellular phenotype of precancerous and cancerous cells of the MCF10A progression series also in a threshold-dependent manner. In particular, AT1 cells restored the apico-basal polarity, indicated by the proper localization of integrin α6 (the basal marker) and cleaved caspase 3 (a marker of lumens)24,135 analogous to non-malignant MCF10A cells (Supplementary Fig. 9A,B). In DCIS and CA1d cells, apico-basal polarity was only partially restored by sepiapterin treatment (Supplementary Fig. 9A,B). Nevertheless, the expression of CK14 (basal cell marker) and the central localization of CK8/18 (luminal cell marker) were almost completely restored (Supplementary Fig. 9C).

We applied sepiapterin to ex vivo 3D cultured mammary tumors from MMTV-PyMT mice (18 weeks old) and tested for its anti-tumor effects. Sepiapterin greatly reversed the proliferative phenotype of the epithelia and even partially restored normal-like glands within tumors in a week. Nevertheless, it needs to be noted that sepiapterin also significantly elevated the vascular density in tumors in support of a notion that the increase of NO promotes antiogenesis20,136,137 (Fig. 8D).

To test the generality of the effects of sepiapterin on breast cancer cells, we pulse-treated different breast cancer cell lines (basal type: MDA-MB231 and MDA-MB468; luminal type: MCF7 and SKBR3) with a different concentration of sepiapterin (0, 20, or 100 μM) in lrECM cultures. Even after two hours of treatment, both 20 and 100 μM of sepiapterin equally increased NO levels of these cancer cell lines by 2~3-fold (Supplementary Fig. 10A). Surprisingly, sepiapterin decreased Ki67 positivity of cancer cells by 60~100% (luminal cells showed better responsiveness than basal cells) (Supplementary Fig. 10B). This result augments a previous report of the growth-inhibitory effects of sepiapterin on breast cancer cells in culture and in animals after 2 days of treatment49.

As a complementary approach, we administered a low concentration (2.5 μM) of a NO donor, SNAP or GSNO, to another breast cancer progression series, HMT-3522 S1 (non-malignant) and T4-2 cells (malignant)24,68,69, cultivated in 3D ECM. This concentration of NO donors were chosen in an attempt to induce production of the physiological level (1–4 μM) of NO previously reported by us and others24,138,139. Similar to sepiapterin, NO donors at 2.5 μM significantly inhibited growth of tumor cells and restored their apico-basal polarity to the level analogous to that of non-malignant cells (Supplementary Fig. 11A–C). To test whether these effects of NO donors are dose-dependent, we administered a different concentration of SNAP or GSNO (0, 2.5 or 10 μM) to the HMT-3522 progression series cultivated in 3D lrECM. Interestingly, while the lower level (2.5 μM) of SNAP and GSNO restored the S1 cell-like polarity and growth-arrested phenotype in T4-2 cells, the higher level (10 μM) of the same NO donors showed no such effects (Supplementary Fig. 12A–C). This result is in line with the well-documented concentration dependence of NO’s bioactivities in cancer17,18,19,20.

The findings altogether suggest that normalization of basal NO level may have a therapeutic potential for breast cancer.

Discussion

Advances in imaging and screening technologies have enabled the detection of precancerous, early-stage breast lesions, the majority of which are ductal carcinoma in situ (DCIS)2. Precancerous lesions arise from clonal expansion of a single cell140. Precancerous lesions are the precursors to invasive breast cancers, and about 40% of them could progress to invasive forms, if untreated2. It is, however, not fully understood what drives formation of precancerous breast lesions, making the management of the disease challenging2.

In the study, we hypothesized that aberrant NO production might contribute to the formation of precancerous breast lesions and tested this possibility. Utilizing the MCF10A breast cancer progression series, we showed that the basal NO level in MECs plummeted along with breast cancer progression, consistent with our previous finding using another breast cancer progression series, HMT-352224. In particular, such decline was the most notable in non-malignant to precancerous transition (Fig. 1A). Reduction of basal level of NO in MECs along with cancer progression was largely attributed to reduction of the NOS cofactor BH4 under increased oxidative stress (Fig. 3B–D). In contrast, the levels of NOS-1 and -3, the enzymes responsible for production of the basal level of NO in the breast, remained unchanged during cancer progression and, thus, were irrelevant to reduction of NO (Fig. 2A).

To confirm the pathological relevance of reduced basal NO production to breast carcinogenesis, we pharmacologically inhibited NO production in prepubertal to pubertal mice using L-NAME, an unreactive L-arginine analog. Previous studies report somewhat conflicting observations for the effects of L-NAME on cancer. Some studies report anti-cancer effects of L-NAME on already established cancer cells141,142,143, while others report the opposite144,145,146,147. Such discrepancy may reflect the complex activities of NO and NOS in cancer18,20,24,35,36,37,38,39,40,41,42,43,47,48,49,50,145,148,149 as well as possible co-suppression of NOS and arginase by L-NAME at high concentrations (>5 mM)84,85,150. L-NAME’s effect on the pathophysiology of normal cells, on the other hand, has yet to be explored.

L-NAME treatment of developing mouse mammary glands impaired alveologenesis, inducing precancerous lesions and desmoplastic ECM (Fig. 4A–C). Consistently, these mammary glands showed overactivation of ERBB2, closely linked to formation of precancerous lesions100,101, and fibrogenic TGFβ (Fig. 4B,D)97. Activation of these pathways were accompanied by the induction of senescence and stem cell-like properties, both prevalent in precancerous lesions (Figs 4D, 6B)59,62,63,101. We further showed that normalization of NO levels, by the use of the BH4 precursor (sepiapterin) or the physiological level of NO donor (SNAP or GSNO), suppressed TGFβ and ERBB2 signals and ameliorated the malignant phenotype of precancerous and cancerous MECs (Fig. 8A–D, Supplementary Fig. 11A–C).

NO’s bioactivities are largely dependent on its concentration, timing and context17,18,19. In healthy tissues, NO production is tightly regulated to attain the right condition151. In disease states, on the other hand, NO production is often dysregulated, leading to a deficient or excessive level of NO that, in either case, could contribute to the disease pathogenesis39,40. Such a complex, paradoxical role of NO in disease conditions, especially in cancer, have led to conflicting reports and a notion that NO plays a double-edged role as both a cancer-promoter and -inhibitor17,18,20. The enigma of NO’s role in cancer might be partly resolved by clarifying how NO is involved in a specific stage of a particular type of cancer under a certain context.

The present study demonstrates that maintenance of the physiological NO level in the breast exerts protective effects against formation of precancerous lesions. NO production, however, could be impaired by oxidative stress that depletes the NOS cofactor BH4, contributing to pathogenesis. Under such a condition, NOS is dysfunctional (uncoupled) and produces superoxide instead of NO, exacerbating oxidative stress49,88. In line with this notion, we observed that NO and BH4 levels both dramatically declined along with an increase in oxidative stress in precancerous and cancerous MECs cultivated in 3D lrECM (Figs 1A and 3B–D).

One of the most compelling findings in this study is that NO deprivation simultaneously upregulated TGFβ and ERBB2 in MECs both in vivo and in vitro (Figs 4B,D and 5A,B). TGFβ and ERBB2 are both under tight regulation in healthy tissues, whereas they become dysregulated during carcinogenesis152,153. TGFβ activity is primarily regulated post-translationally, especially through formation of the latent complex along with LTBP1 and LAP154. ERBB2 elevation, in contrast, is primarily ascribed to gene amplification155. However, other mechanisms that do not involve changes in DNA sequence also play major roles in regulation of ERBB2 level. These mechanisms include transcriptional and post-transcriptional activation156,157,158 as well as protein stabilization159. In fact, it is shown that ~20% of ERBB2-positive tumors detected by IHC (score of 3+) do not harbor amplification of the ERBB2 gene160,161. We are postulating that the basal steady-state level of NO produced in the healthy breast tissue might negatively regulate proteins involved in upregulation of TGFβ and ERBB2 via S-nitrosylation (SNO). SNO plays a large part of NO signal, regulating structures and functions of >3000 proteins162. In healthy cells, a subset of proteins are constitutively S-nitrosylated at the basal level to remain under control25. In disease states including cancer, on the other hand, SNO level could be dysregulated, contributing to disruption of homeostasis25. Currently, we are examining the potential role of SNO in suppressing TGFβ and ERBB2 expression and activity in non-malignant MECs.

Our study demonstrates that normalization of NO level with the BH4 precursor, sepiapterin (20 or 100 μM), or with a low level (2.5 μM) of a NO donor, SNAP or GSNO, reduced ERBB2 and TGFβ signals and suppressed the proliferative phenotype of precancerous and cancerous MECs in 3D lrECM. NO normalization also restored cell polarity and lineage markers in these cells (a process termed ‘phenotypic reversion’24) (Fig. 8, Supplementary Figs 812). Surprisingly, application of sepiapterin to ex vivo 3D cultured mammary tumors partially restored normal-like glands and largely reversed the proliferative phenotype of tumor epithelia in a week (Fig. 8D). However, it is critical to note that modulation of NO levels should aim at restoring the physiological basal level of NO (1–4 μM) in MECs24,138,139. Too much or too little NO supplementation, on the other hand, could result in pathogenic effects because of the concentration-dependent NO’s bioactivities18,20. In fact, while NO donors at the lower concentration (2.5 μM) exerted anti-cancer activity, the same donors at the higher concentration (10 μM) showed no such activity (Supplementary Fig. 12A–C). In contrast, sepiapterin exerted the anti-cancer activity equally at both 20 and 100 μM, and thus was threshold-dependent at least within this range. These results suggest that sepiapterin might have a wider therapeutic window than NO donors.

Our present findings strongly suggest the translational potentials of sepiapterin (and possibly the physiological concentrations of NO donors) for treatment of early-stage breast cancer. However, the advancement of such approach would depend on the development of tumor-restricted drug delivery systems, because systemic administration of these agents could have potential drawbacks17,163,164,165. While systemic administration of sepiapterin to animals is shown to reduce tumor cell proliferation49, it also enhances vascularization of tumor tissues20,136,137. Consistently, when we applied sepiapterin to ex vivo 3D cultured mouse mammary tumors, their proliferative phenotype was dramatically suppressed, whereas the vasculature was significantly enhanced (Fig. 8D). Such enhanced vasculature by sepiapterin treatment might eventually help tumor cells re-grow and reduce the efficacy of the drug. To circumvent these drawbacks, we are currently developing liposome-based systems that could specifically deliver sepiapterin to the breast epithelia of lesions via specific homing peptides166. Moreover, future studies could possibly determine whether certain diet and exercise routines help maintain the physiological NO level in the breast and prevent formation of precancerous lesions.

Materials and Methods

Cell lines

Cell lines of the MCF10A breast cancer progression series were obtained from Karmanos Cancer Institute (MI, USA)78 under Material Transfer Agreement. Cell lines of the HMT-3522 breast cancer progression series (S1 and T4-2) were provided by Mina Bissell laboratory in Lawrence Berkeley National Laboratory (Berkeley, CA)24 under Material Transfer Agreement. All the other breast cancer cell lines were obtained from American Tissue Culture Collection (ATCC). All the cell lines had been authenticated by the providers through genome sequencing and STR profiling. Mycoplasma testing of these cell lines was negative.

Cell culture and reagents

The MCF10A breast cancer progression series comprising non-malignant MCF10A, premalignant AT1, in situ carcinoma DCIS.COM and metastatic CA1d, was maintained as described78. The isogenic cell lines of the HMT-3522 human breast cancer progression series, comprising non-malignant S1 and malignant T4-2 cells, were maintained as described previously24. All the other breast cancer cell lines were maintained in DMEM/F12 with 10% FBS and 1% penicillin/streptomycin. For 3D culture experiments, cells were seeded at the density of 2.5 × 104 cells/cm2 for non-malignant cells and 1.8 × 104 cells/cm2 for malignant cells in growth factor reduced Matrigel (BD Biosciences) and maintained for 10–21 days with addition of fresh medium on alternate days. For inhibition of NO production, cells were treated with 2.5 mM L-NAME (Nω-Nitro-L-arginine methyl ester hydrochloride, Sigma- Aldrich); for induction of NO production, 2.5 or 10 μM SNAP (S-Nitroso-N-acetyl-DL-penicillamine,) or 2.5 or 10 μM GSNO (S-nitrosoglutathione, Sigma-Aldrich) was used. To compensate for the reduced BH4 level in cancer cells, 20 or 100 μM L-sepiapterin (BH4 precursor, Sigma-Aldrich) was used. The NOS inhibitors were all obtained from Cayman Chemical. NOS1 inhibitor (Nω-Propyl-L-arginine hydrochloride) was used at 10 µM; NOS2 inhibitor (1400 W) at 50 µM; and NOS3 inhibitor (L-NIO) at 10 µM167.

Antibodies

The following antibodies were used. Anti-β-Galactosidase (Bioss, bs-4960R), anti-alkaline phosphatase (Novus Biologicals, NBP1-32948); anti-heterochromatin protein 1-γ (HP1-γ, phospho Ser 93, Bioss, bs-3221R); anti-p21 (Bioss, bs-10129R); anti-p27 (phospho Thr 187, Abcam, ab75908); anti-NOS-1, 2 (Thermo Fisher Scientific, PA1-033 and -036); anti-NOS-3 (Sigma-Aldrich, SAB-4300435); anti-ErbB2 (Thermo Fisher Scientific, PA5-16395); anti-pSMAD3 (Ser423/Ser425, Novous Biological, NBP1-77836); anti-CD24 (Novus Biologicals, NBP1-4639055); anti-CD44 (Bioss, bs-2507R); anti-S-Nitroso-Cysteine (Abcam, ab50185 or Alpha Diagnostics, NISC11-A); anti-Integrin α6 (BD Biosciences, 555734); anti-GM130 (Cell Signaling, 12480 S); anti-human CK 14 (ThermoFisher, MA511599); anti-human CK 18 (ThermoFisher, PA514263); anti-mouse CK 14 (BioLegend, 905301); anti-human CK 8/18 (DSHB, Troma-I); anti-Cleaved Caspase3 (Cell Signaling, #9664); anti-β-Actin (Sigma, A1978); anti-DYNLL1 (Abcam, ab51603); and anti-ADMA (EMD Millipore, 09-814).

NO measurement in live cells

To capture the snap shot of NO production in live cells after Matrigel addition, a dye DAF-FM DA (4-Amino-5-Methylamino-2′,7′-Difluorofluorescein Diacetate, Life Technologies) was used according to the manufacturer’s protocol. Briefly, cells were seeded at 1.0 × 105 cells/24 well-plate maintained in phenol red free growth media overnight and pre-treated with the dye for 1 h. After the drip (5%) of Matrigel (phenol red-free) was added, cells were incubated in dark for 1 h and washed in fresh media. Micrographs were taken on live cells by fluorescent microscope with FITC filter, and the signal intensity/cell was measured with ImageJ.

Nitrite measurement

To quantify the cumulative level of nitric oxide produced by cells, more stable nitric oxide metabolite, nitrite, was measured based on the reaction of a dye DAN (diaminonaphthalene) by using Measure-IT High-Sensitivity Nitrite Assay Kit (Life technologies), according to the manufacturer’s protocol. Briefly, cells were plated at 1 × 106 cells/60 mm-plate and maintained overnight. Cells were maintained in 2 ml of the fresh phenol red-free medium containing 5% Matrigel (phenol red-free, Corning, #356237) for 24 h. The conditioned medium was harvested and spun to remove the Matrigel. Ten μl of the cleared conditioned medium was reacted with the assay reagents in dark, and the signal intensity was measured using nitrite standards at the excitation/emission maxima of 340/410 nm.

pH measurement

The pH of cell lines of the MCF10A progression series were measured with the pHrodo® Green AM Intracellular pH Indicator (Cat# P35373, Thermo Fisher Scientific) according to the manufacturer’s protocol. Briefly, live cells were incubated with the pH probe for 30 min. For standard samples, the standard solution (Cat# P35379, Thermo Fisher Scientific) for each different pH was added at the end of 30 min, and cells were incubated for another 5 min. Cells were washed in fresh media, and micrographs were taken on live cells by fluorescent microscope with FITC filter. The signal intensity per cell was quantified by ImageJ.

Measurement of oxidative stress

Oxidative stress in cell lines of the MCF10A progression series was determined with Cellular ROS/Superoxide Detection Assay Kit (ab139476, Abcam), which measures total reactive oxygen species and superoxide separately, according to the manufacturer’s protocol. The total ROS level was measured on plate reader with fluorescein filter set. For determination of superoxide signal, micrographs were taken on live cells by fluorescent microscope with Texas Red filter, and the signal intensity per cell was quantified by ImageJ.

BH4 measurement

Cell lines of the MCF10A progression series were cultured until they became confluent in T-175 flasks. After trypsinization, cells were washed 3 times in cold PBS and pelleted. Intercellular BH4 levels were measured by the ELISA kit (abx519576, ABBEXA, UK) according to the manufacture’s protocol. Protein concentration and cell number were normalized in the provided sample buffer across the cell lines. The signal intensity was measured in triplicates for each sample at 450 nm.

NOS knockdown by shRNA

To knock-down each NOS isoform, lentiviral NOS shRNA vectors that target respective sequences were obtained from Origene (Supplementary Table 1). As a control, lentiviral vector that expresses scramble sequence (CAT No: TR30021) was used. Lentiviral particles were produced as described below and applied to MCF10A cells to make stable cell lines.

Lentivirus production and transduction

Lentivirus production and transduction of target cells were conducted following the guideline by Origene. Briefly, lentivirus vector and packaging plasmid mix (Origene) were transfected into 293FT cells (Invitrogen) using Lipofectamine® 3000. After 48 hrs, medium was harvested, filtered and used to infect target cells with the addition of polybrene (10 μg/ml). After 24 hrs, medium was replaced. At 72 hrs post-infection, puromycin (0.5 μg/ml) was added for selection and maintained throughout the culturing period.

NOS knockdown by siRNA

To simultaneously knockdown two NOS isoforms, MCF10A cells expressing NOS1-3 shRNA were transfected with NOS1-3 siRNA (Dharmacon, Supplementary Table 2) using Lipofectamine® RNAiMAX Transfection Reagent (ThermoFisher) according to the manufacturer’s guideline.

Immunohistochemistry

To determine the expression of specific markers, paraffin-embedded sections of mouse mammary tissues were analyzed by immunohistochemistry. Briefly, sections were deparaffinized, hydrated, and treated with antigen unmasking solutions (Vector Laboratories, Inc.) or with Tris-EDTA Buffer (10 mM Tris Base, 1 mM EDTA Solution, 0.05% Tween 20, pH 9.0) heated to 95–100 °C in a pressure cooker. After being blocked with nonimmune goat serum, sections were processed for immunofluorescence staining as described below.

Immunofluorescence staining and imaging

Immunofluorescence staining/imaging was performed as described previously24. Samples were incubated with primary antibody for overnight at 4 degree in a humidified chamber. After intensive washing (three times, 15 min each) in 0.1% BSA, 0.2% Triton-X 100, 0.05% Tween 20, 0.05% NaN3 in PBS, fluorescence-conjugated secondary antibodies (Molecular Probes) were added for 1 hr at room temperature. Nuclei were stained with 0.5 ng/ml DAPI. After mounted with anti-fade solution, epi-fluorescence imaging was performed on Olympus IX70 microscope using CellSens software. Confocal fluorescence imaging with Second Harmonics Generation (SHG) module96 was performed on Leica Microsystems TCS SP5 multi-photon laser scanning confocal microscope using Suite Advanced Fluorescence (LAS AF) software.

Image Analysis

Quantification of fluorescence signal in micrographs was performed with ImageJ software (NIH) referring to the owner’s manual (http://imagej.net/docs/guide/146.html). Briefly, a region of interest (ROI) was determined in reference to an image of DAPI-stained nuclei. For quantification of signal in individual cultured cells, the whole cell was selected as ROI. For quantification of signal in individual organoids in cultures or tissues, each organoid was selected as ROI. For quantification of second harmonics generation (SHG) signal in mammary tissues, the ROI was defined as the periductal ECM/stromal area between the epithelial and adipose layers. For quantification of S-NOC signal in mammary tissues, epithelial layers were selected by setting a threshold range, and the intensity was measured for each gland. For each ROI, the average intensity per pixel was measured, and background intensity was subtracted. For each sample group, at least 50 to 200 measurements were performed. Furthermore, measurement of each sample set was repeated by at least three people, and the results were combined for the final data. The mean value was represented as arbitrary units (AU). The statistical significance of the data was further evaluated using Graphpad Prism Version 5 software (see statistics section).

Animal Studies

All animal experiments conformed to The Guide for the Care and Use of Laboratory Animals (National Research Council, National Academy Press, Washington, D.C., 2010) and were performed with the approval of the Institutional Animal Care and. Use Committee of the University of Toledo, Toledo, OH (Protocol No: 108658). Three-weeks old female BALB/c (n = 18) mice were obtained from the Jackson Laboratory (Bar Harhor, MN) and housed under a 12 hr light-dark cycle and given regular chow. Starting at the age of 4 weeks old, mice were given intraperitoneal injection of either drug (vehicle: PBS (100 µl), L-arginine (20 mg/kg, 100 µl), or L-NAME (20 mg/kg, 100 µl)) every other day for 6 weeks. Body weight and morbidity of animals were monitored throughout the treatment period. At the end of treatment period, mice were euthanized, and inguinal mammary glands were harvested. Number 4 mammary glands were processed for whole mounting as described168, while number 5 glands were processed for paraffin-embedding and sectioning. Whole mount was imaged by Cytation5 Cell Imaging Multi-Mode Reader (BioTech Instruments). To determine the gross morphology of glands, paraffin sections were deparaffinized, hydrated and stained with eosin/hematoxyline. Other sections were analyzed by immunohistochemistry and SHG imaging.

Ex Vivo 3D Cultures

Mouse mammary tumors (#4 glands, ~1 cm in diameter, n = 4) were harvested from 18 weeks old female MMTV-PyMT mice (Jackson). Tumors were rinsed in PBS and chopped into ~1 mm × 2 mm × 1 mm fragments, as previously described169,170. 1~2 fragments/48 well were plated onto the ECM gel coat (Matrigel) and cultured in DMEM + 10% FBS + 1% penicillin/streptomycin with 4% Matrigel and sepiapterin (0, 20 or 100 μM) for one week with drug replenishment every 2–3 days. Tumors were fixed, paraffin-embedded, sectioned and stained with eosin/hematoxyline.

Mammosphere assay

MCF10A cell lines were pretreated for 7 days with either vehicle, L-arginine (2.5 mM) or L-NAME (2.5 mM), and then subjected to mammosphere assay as described120,121,129. Briefly, the day before experiment, culture plates were coated with poly-HEMA (#3932, Sigma) as previously described171. Single cell suspension of 4 × 104 cells were resuspended in 2 ml media from Mammocult Human medium kit (#5620, Stemcell Technologies) with 4 μg/ml heparin and 0.48 μg/ml hydrocortisone, and plated into each well of 6-well plates. Media were replaced every other day, and mammospheres were harvested after 7 days and processed for immunostaining/imaging (spheroids in suspension or paraffin-embedded/sectioned129) or FACS analysis (see below). For the mammosphere formation efficiency assay previously described119,120,121,122,123,124, the starting cell density was 10,000 cells per well of 48 well plate (n = 4), and was serially diluted to the level <100 cells per well (10,000, 5000, 2500, 1250, 625, 312, 156, 78; spheres were countable when seeded at the densities ≥1250/48-well for all the treatment groups). After one week of culturing, microscopy images were taken on phase I filter, and spheres larger than 75 μM in diameter were counted using ImageJ. The data are presented as both the number of spheroids formed at each seeding number (Fig. 7C) and mammosphere forming efficiency [(%) = (# of spheroids)/(# of cells seeded) × 100] for each seeding density (Supplementary Fig. 7B)119,120,121,122,123,124. For limiting dilution analysis previously described126, the starting cell density was 1,600 cells per well of 96 well plate (n = 8), and was serially diluted to 200 cells per well. Each well was examined under light microscope and scored as either “ + ” (spheres present) or “−” (no spheres present). The fraction of “−” wells (1 − P) was calculated as the number of “−” wells/total wells for each condition. Ln (fraction of “−” wells) was plotted in the Y-axis against the number cells seeded in the X-axis, where the of best fit was drown to intersect at the origin. The sphere forming frequency corresponds to −(slope) of the line (see the equation below126).

$${\rm{P}}={\rm{1}}-{{\rm{e}}}^{{\rm{mD}}},{\rm{P}}:{\rm{probably}}\,{\rm{of}}\,{\rm{sphere}}\,{\rm{formation}};{\rm{m}}:{\rm{slope}};{\rm{D}}:{\rm{seeding}}\,{\rm{number}}$$
$$\mathrm{Ln}\,(1-{\rm{P}})=\,\mathrm{Ln}\,(\mathrm{fraction}\,{\rm{of}}\,\mbox{''}-\mathrm{wells})={\rm{mD}}$$
$${\rm{Sphere}}\,{\rm{forming}}\,{\rm{frequency}}=-\,({\rm{slope}})=-{\rm{m}}$$

Flow cytometric (FACS) analysis of mammospheres

FACS analysis of mammospheres was performed as described with slight modifications172. Briefly, mammospheres were collected by centrifugation, resuspended in 200 μL of 1 × 0.25% trypsin-EDTA and incubated for 5 minutes to dissociate cells. Cells were washed and resuspended in the growth medium and rotated at 37 °C in a hybridization oven (15 rpm) for 8 hours to recover cell-surface components173. 1 × 105 cells (100 μl in PBS) were incubated with 1 μg of anti-CD44 and anti-CD24 antibodies or isotype control, followed by the respective fluorophore-conjugated secondary antibodies at room temperature. Cells were collected by centrifugation and resuspended in PBS + BSA (1%) before loading onto BD Biosciences FACSARIA IIU operated with BD FACSDIVA software. The fluorescein isothiocyanate (FITC) was excited at 488 nm and emission recorded in the 530/30 filter channel, while Alexa Fluor 594 fluorophore was excited at 488 nm and emission recorded in the 610/20 filter channel. Compensation values for FITC and Alexa Fluor 594 fluorescence overlap were established using compensation controls and copied to all subsequent analyses. A total of 1000 events were recorded for each sample. Isotype controls were used to set threshold gates.

Statistics

All the experiments were performed in replicates (n > = 3 for in vitro experiments; n > 6 for in vivo experiments) ensuring the adequate statistical power as done previously174. Unless otherwise indicated, statistical significance of the mean difference was tested by two-tailed t-tests (parametric) using Graphpad Prism Version 5 software. P-values of 0.05 or less were considered significant. Average results of multiple experiments (n > = 3) are presented as the arithmetic mean ± SEM.

References

  1. 1.

    Siegel, R. L., Miller, K. D. & Jemal, A. Cancer statistics, 2018. CA Cancer J Clin 68, 7–30 (2018).

  2. 2.

    Sgroi, D. C. Preinvasive breast cancer. Annu Rev Pathol 5, 193–221 (2010).

  3. 3.

    Zhao, Y. et al. Pubertal high fat diet: effects on mammary cancer development. Breast Cancer Res. 15, R100 (2013).

  4. 4.

    Wu, Y., Zhang, D. & S, K. Physical activity and risk of breast cancer: a meta-analysis of prospective studies. Breast Cancer Res Treat 137, 869–882 (2013).

  5. 5.

    Novosyadlyy, R. et al. Insulin-mediated acceleration of breast cancer development and progression in a nonobese model of type 2 diabetes. Cancer Res. 70, 741–751 (2010).

  6. 6.

    Stoll, B. Adiposity as a risk determinant for postmenopausal breast cancer. Int J Obes Relat Metab Disord 24, 527–533 (2000).

  7. 7.

    Stoll, B. Alcohol intake and late-stage promotion of breast cancer. Eur J Cancer 35, 1653–1658 (1999).

  8. 8.

    Catsburg, C., Miller, A. B. & Rohan, T. E. Active cigarette smoking and risk of breast cancer. Int J Cancer 136, 2204–2209 (2015).

  9. 9.

    Han, H. et al. Hypertension and breast cancer risk: a systematic review and meta-analysis. Sci Rep. 7, 44877 (2017).

  10. 10.

    Martins, M. A. et al. High fat diets modulate nitric oxide biosynthesis and antioxidant defence in red blood cells from C57BL/6 mice. Arch Biochem Biophys 499, 56–61 (2010).

  11. 11.

    Afsharm, M. et al. Exhaled Nitric Oxide Levels Among Adults With Excessive Alcohol Consumption. Chest 150, 196–209 (2016).

  12. 12.

    Nyberg, M. et al. Lifelong physical activity prevents an age-related reduction in arterial and skeletal muscle nitric oxide bioavailability in humans. J Physiol 590, 5361–5370 (2012).

  13. 13.

    Tessari, P. et al. Nitric oxide synthesis is reduced in subjects with type 2 diabetes and nephropathy. Diabetes 59, 2152–2159 (2010).

  14. 14.

    Williams, I., Wheatcroft, S. B., Shah, A. M. & Kearney, M. T. Obesity, atherosclerosis and the vascular endothelium: mechanisms of reduced nitric oxide bioavailability in obese humans. Int J Obes Relat Metab Disord 26, 754–764 (2002).

  15. 15.

    Bodis, S. & Haregewoin, A. Significantly reduced salivary nitric oxide levels in smokers. Ann Oncol 5, 371–372 (1994).

  16. 16.

    Panza, J. A., Casino, P. R., Kilcoyne, C. M. & Quyyumi, A. A. Role of endothelium-derived nitric oxide in the abnormal endothelium-dependent vascular relaxation of patients with essential hypertension. Circulation 87, 1468–1474 (1993).

  17. 17.

    Scicinski, J. et al. NO to cancer: The complex and multifaceted role of nitric oxide and the epigenetic nitric oxide donor, RRx-001. Redox Biol. 6, 1–8 (2015).

  18. 18.

    Choudhari, S. K., Chaudhary, M., Sachin, Gadbail, A. R. & Joshi, V. Nitric oxide and cancer: a review. World J Surg Oncol 11, 118 (2013).

  19. 19.

    Thomas, D. D. et al. Hypoxic inducible factor 1alpha, extracellular signal-regulated kinase, and p53 are regulated by distinct threshold concentrations of nitric oxide. Pro Natl Acad Sci USA 101, 8894–8899 (2004).

  20. 20.

    Burke, A. J., Sullivan, F. J., Giles, F. J. & Glynn, S. A. The yin and yang of nitric oxide in cancer progression. Carcinogenesis 34, 503–512 (2013).

  21. 21.

    Antosova, M., Plevkova, J., Strapkova, A. & Buday, T. Nitric oxide—Important messenger in human body. OJMIP 2, 98–106 (2012).

  22. 22.

    López-Figueroa, M. O. et al. Characterization of basal nitric oxide production in living cells. Biochim Biophys Acta 1540, 253–264 (2001).

  23. 23.

    Young, S. L., Evans, K. & Eu, J. P. Nitric oxide modulates branching morphogenesis in fetal rat lung explants. Am J Physiol Lung Cell Mol Physiol. 282, L379–385 (2002).

  24. 24.

    Furuta, S., Ren, G., Mao, J. & Bissell, M. J. Laminin signals initiate the reciprocal loop that informs breast-specific gene expression and homeostasis by activating NO, p53 and microRNA. eLife 7, e26148 (2018).

  25. 25.

    Furuta, S. Basal S-nitrosylation is the guardian of tissue homeostasis. Trends in Cancer 3, 744–748. PMID: 29120749 (2017).

  26. 26.

    Islam, M. S. et al. Immunohistochemical localization of nitric oxide synthase (NOS) in mouse mammary gland during reproductive cycle. J Vet Med Sci 71, 945–949 (2009).

  27. 27.

    Iizuka, T., Sasaki, M., Oishi, K., Uemura, S. & Koike, M. The Presence of Nitric Oxide Synthase in the Mammary Glands of Lactating Rats. Pediatric Research 44, 197 (1998).

  28. 28.

    Wockel, A. et al. Constitutive coexpression of nitric oxide synthase-1 and soluble guanylyl cyclase in myoepithelial cells of mammary glands in mice. Cells Tissues Organs 180, 174–184 (2005).

  29. 29.

    Akçay, F., Aksoy, H. & Memisoğullari, R. Effect of breast-feeding on concentration of nitric oxide in breast milk. Ann Clin Biochem. 39, 68–69 (2002).

  30. 30.

    Iizuka, T. et al. Nitric oxide may trigger lactation in humans. J Pediatr. 131, 839–843 (1997).

  31. 31.

    Alkareem, M. A., AlBayati, M. A. & Khamas, W. The effect of L-arginine and antagonist L-NAME on the mammary gland of pregnant mice. JPCS 6, 36–37 (2013).

  32. 32.

    Kim, S. W. & Wu, G. Regulatory role for amino acids in mammary gland growth and milk synthesis. Amino Acids 37, 89–95 (2009).

  33. 33.

    Tezer, M., Ozluk, Y., Sanli, O., Asoglu, O. & Kadioglu, A. Nitric oxide may mediate nipple erection. J. Androl. 33, 805–810 (2012).

  34. 34.

    Hord, N. G., Ghannam, J. S., Garg, H. K., Berens, P. D. & Bryan, N. S. Nitrate and nitrite content of human, formula, bovine, and soy milks: implications for dietary nitrite and nitrate recommendations. Breastfeed Med. 6, 393–399 (2011).

  35. 35.

    Thomsen, L. L. et al. Nitric oxide synthase activity in human breast cancer. Br J Cancer 72, 41–44.

  36. 36.

    Sangle, V. A. et al. Elevated tissue nitric oxide in oral squamous cell carcinoma. J Oral Maxillofac Pathol 22, 35–39 (2018).

  37. 37.

    Abdel-Salam, O., Youness, E. & Hafez, H. The antioxidant status of the plasma in patients with breast cancer undergoing chemotherapy. Open Journal of Molecular and Integrative Physiology 1, 29–35 (2011).

  38. 38.

    Simeone, A. M., Broemeling, L. D., Rosenblum, J. & Tari, A. M. HER2/neu reduces the apoptotic effects of N-(4-hydroxyphenyl)retinamide (4-HPR) in breast cancer cells by decreasing nitric oxide production. Oncogene 22, 6739–6747 (2003).

  39. 39.

    Janakiram, N. B. & Rao, C. V. In Nitric Oxide and Cancer: Pathogenesis and Therapy 159–175 (Springer International Publishing, 2015).

  40. 40.

    Schulz, G. & Stechmiller, J. Wound healing and nitric oxide production: too little or too much may impair healing and cause chronic wounds. Int J Low Extrem Wound 5, 6–8 (2006).

  41. 41.

    Hickok, J. R. & Thomas, D. D. Nitric oxide and cancer therapy: the emperor has NO clothes. Curr Pharm Des 16, 381–391 (2010).

  42. 42.

    Ridnour, L. A. et al. Molecular mechanisms for discrete nitric oxide levels in cancer. Nitric Oxide 19, 73–76 (2000).

  43. 43.

    Vannini, F., Kashfi, K. & Nath, N. The dual role of iNOS in cancer. Redox Biol 6, 334–343 (2015).

  44. 44.

    Zheng, X. et al. Redirecting tumor-associated macrophages to become tumoricidal effectors as a novel strategy for cancer therapy. Oncotarget 8, 48436–48452 (2017).

  45. 45.

    Xu, W., Liu, L. Z., Loizidou, M., Ahmed, M. & Charles, I. G. The role of nitric oxide in cancer. Cell Research 12, 311–320 (2002).

  46. 46.

    Cai, S., Khoo, J. & Channon, K. M. Augmented BH4 by gene transfer restores nitric oxide synthase function in hyperglycemic human endothelial cells. Cardiovasc Res 65, 823–831 (2005).

  47. 47.

    Santhanam, A. V., d’Uscio, L. V., Smith, L. A. & Katusic, Z. S. Uncoupling of eNOS causes superoxide anion production and impairs NO signaling in the cerebral microvessels of hph-1 mice. J Neurochem 122, v (2012).

  48. 48.

    Melo, F. H. et al. Endothelial nitric oxide synthase uncoupling as a key mediator of melanocyte malignant transformation associated with sustained stress conditions. Free Radic Biol Med 50, 1263–1273 (2011).

  49. 49.

    Rabender, C. S. et al. The Role of Nitric Oxide Synthase Uncoupling in Tumor Progression. Mol Cancer Res. 13, 1034–1043 (2015).

  50. 50.

    Jo, H. et al. Inhibition of nitric oxide synthase uncoupling by sepiapterin improves left ventricular function in streptozotocin-induced diabetic mice. Clin Exp Pharmacol Physio 38, 485–493 (2011).

  51. 51.

    Ambs, S. et al. Up-regulation of inducible nitric oxide synthase expression in cancer-prone p53 knockout mice. Proc. Nat. Acad Sci USA 95, 8823–8828 (1998).

  52. 52.

    Vakkala, M. et al. Inducible Nitric Oxide Synthase Expression, Apoptosis, and Angiogenesis in in Situ and Invasive Breast Carcinomas. Clinical Cancer Research 6, 2408–2416 (2000).

  53. 53.

    Ricca, B. L. et al. Transient external force induces phenotypic reversion of malignant epithelial structures via nitric oxide signaling. Elife 7, e26161 PMCID: PMC5862525 (2018).

  54. 54.

    Haagensen, C. D. Diseases of the Breast, 3rd Ed., (WB Saunders Co., 1986).

  55. 55.

    Ohuchi, N., Abe, R. & Kasai, M. Possible cancerous change of intraductal papillomas of the breast. A 3-D reconstruction study of 25 cases. Cancer 54, 605–611 (1984).

  56. 56.

    Harjit, K. et al. Multiple papillomas of the breast: is current management adequate? Breast 15, 777–781 (2006).

  57. 57.

    Debnath, D., Al-Okati, D. & Ismail, W. Multiple Papillomatosis of Breast and Patient’s Choice of Treatment. Patholog Res Int. 2010, 540590 (2010).

  58. 58.

    Al Sarakbi, W., Worku, D., Escobar, P. F. & Mokbel, K. Breast papillomas: current management with a focus on a new diagnostic and therapeutic modality. Int. Semin Surg. Oncol. 3, 1 (2006).

  59. 59.

    Collado, M. et al. Tumour biology: senescence in premalignant tumours. Nature 436, 642 (2005).

  60. 60.

    Collado, M. & Serrano, M. The power and the promise of oncogene-induced senescence markers. Nat Rev Cancer 6, 472–476 (2006).

  61. 61.

    Collado, M. & Serrano, M. Senescence in tumours: evidence from mice and humans. Nat Rev Cancer 10, 51–57 (2010).

  62. 62.

    Damonte, P. et al. Mammary carcinoma behavior is programmed in the precancer stem cell. Breast Cancer Res. 10, R50 (2008).

  63. 63.

    Chen, L. et al. Precancerous stem cells have the potential for both benign and malignant differentiation. PLoS One 2, e293 (2007).

  64. 64.

    Gao, J. X. Cancer stem cells: the lessons from pre-cancerous stem cells. J Cell Mol Med. 12, 67–96 (2008).

  65. 65.

    Gloe, T., Riedmayr, S., Sohn, H.-Y. & Pohl, U. The 67-kDa Laminin-binding Protein Is Involved in Shear Stress-dependent Endothelial Nitric-oxide Synthase Expression. Journal of Biological Chemistry 274, 15996–16002, https://doi.org/10.1074/jbc.274.23.15996 (1999).

  66. 66.

    Hou, L., Coller, J., Natu, V., Hastie, T. J. & Huang, N. F. Combinatorial extracellular matrix microenvironments promote survival and phenotype of human induced pluripotent stem cell-derived endothelial cells in hypoxia. Acta Biomater 44, 188–199 (2016).

  67. 67.

    Moon, T. C., Yoshimura, T., Parsons, T. & Befus, A. D. Microenvironmental regulation of inducible nitric oxide synthase expression and nitric oxide production in mouse bone marrow-derived mast cells. J Leukoc Biol. 91, 581–590 (2012).

  68. 68.

    Briand, P., Petersen, O. W. & Van Deurs, B. A new diploid nontumorigenic human breast epithelial cell line isolated and propagated in chemically defined medium. In Vitro Cell Dev Biol 23, 181–188 (1987).

  69. 69.

    Briand, P., Nielsen, K. V., Madsen, M. W. & Petersen, O. W. Trisomy 7p and malignant transformation of human breast epithelial cells following epidermal growth factor withdrawal. Cancer Res 56, 2039–2044 (1996).

  70. 70.

    Moyret, C., Madsen, M. W., Cooke, J., Briand, P. & Theillet, C. Gradual selection of a cellular clone presenting a mutation at codon 179 of the p53 gene during establishment of the immortalized human breast epithelial cell line HMT-3522. Exp Cell Res 215, 380–385 (1994).

  71. 71.

    Vidi, P. A., Bissell, M. J. & Lelièvre, S. A. Three-dimensional culture of human breast epithelial cells: the how and the why. Methods Mol Biol. 945 (2013).

  72. 72.

    Rizki, A. et al. A human breast cell model of preinvasive to invasive transition. Cancer Res. 68, 1378–1387 (2008).

  73. 73.

    Briand, P. & Lykkesfeldt, A. E. An in vitro model of human breast carcinogenesis: epigenetic aspects. Breast Cancer Res Treat 65, 179–187 (2001).

  74. 74.

    Soule, H. D. et al. Isolation and characterization of a spontaneously immortalized human breast epithelial cell line, MCF-10. Cancer Res. 50, 6075–6086 (1990).

  75. 75.

    Pauley, R. J. et al. The MCF10 family of spontaneously immortalized human breast epithelial cell lines: models of neoplastic progression. Eur J Cancer Prev 2, 67–76 (1993).

  76. 76.

    Heppner, G. H. & Wolman, S. R. MCF-10AT: A Model for Human Breast Cancer Development. Breast J 5, 122–129 (1999).

  77. 77.

    Miller, F. R., Santner, S. J., Tait, L. & Dawson, P. J. MCF10DCIS.com xenograft model of human comedo ductal carcinoma in situ. J Natl Cancer Inst. 92, 1185–1186 (2000).

  78. 78.

    Santner, S. J. et al. Malignant MCF10CA1 cell lines derived from premalignant human breast epithelial MCF10AT cells. Breast Cancer Res Treat 65, 101–110 (2001).

  79. 79.

    Li, Q., Mullins, S. R., Sloane, B. F. & Mattingly, R. R. p21-Activated kinase 1 coordinates aberrant cell survival and pericellular proteolysis in a three-dimensional culture model for premalignant progression of human breast cancer. Neoplasia 10, 314–329 (2008).

  80. 80.

    Imbalzano, K. M., Tatarkova, I., Imbalzano, A. N. & Nickerson, J. A. Increasingly transformed MCF-10A cells have a progressively tumor-like phenotype in three-dimensional basement membrane culture. Cancer Cell Int. 9, 7 (2009).

  81. 81.

    Nott, A., Robinson, J. D. & Riccio, A. DAF-FM detection of nitric oxide in embryonic cortical neurons (2008).

  82. 82.

    Misko, T. P., Schilling, R. J., Salvemini, D., Moore, W. M. & Currie, M. G. A fluorometric assay for the measurement of nitrite in biological samples. Anal Biochem 214, 11–16 (1993).

  83. 83.

    Pfeiffer, S., Leopold, E., Schmidt, K., Brunner, F. & Mayer, B. Inhibition of nitric oxide synthesis by NG-nitro-L-arginine methyl ester (L-NAME): requirement for bioactivation to the free acid, NG-nitro-L-arginine. Br J Pharmacol 118, 1433–1440 (1996).

  84. 84.

    Robertson, C. A., Green, B. G., Niedzwiecki, L., Harrison, R. K. & Grant, S. K. Effect of nitric oxide synthase substrate analog inhibitors on rat liver arginase. Biochem Biophys Res Commun. 197, 523–528 (1993).

  85. 85.

    Reisser, D., Onier-Cherix, N. & Jeannin, J. F. Arginase activity is inhibited by L-NAME, both in vitro and in vivo. J Enzyme Inhib Med Chem 17, 267–270 (2002).

  86. 86.

    Abdelmagid, S. A. & Too, C. K. Prolactin and estrogen up-regulate carboxypeptidase-d to promote nitric oxide production and survival of mcf-7 breast cancer cells. Endocrinology 149, 4821–4828 (2008).

  87. 87.

    Pavlova, N. N. & Thompson, C. B. The Emerging Hallmarks of Cancer Metabolism. Cell Metab 23, 27–47 (2016).

  88. 88.

    Landmesser, U. et al. Oxidation of tetrahydrobiopterin leads to uncoupling of endothelial cell nitric oxide synthase in hypertension. J Clin Invest 111, 1201–1209 (2003).

  89. 89.

    Yaqoob, M. et al. Nitric oxide kinetics during hypoxia in proximal tubules: effects of acidosis and glycine. Kidney Int. 49, 1314–1319 (1996).

  90. 90.

    Conte, A. Role of pH on the calcium ion dependence of the nitric oxide synthase in the carp brain. Brain Res Bull 56, 67–71 (2001).

  91. 91.

    Mas, M. A Close Look at the Endothelium: Its Role in the Regulation of Vasomotor Tone. Euro Urol Suppl 8, 48–57 (2009).

  92. 92.

    Wang, S. C. et al. RNA silencing targeting PIN (protein inhibitor of neuronal nitric oxide synthase) attenuates the development of hypertension in young spontaneously hypertensive rats. J Am Soc Hypertens 8, 5–13 (2014).

  93. 93.

    Kolluru, G. K., Bir, S. C. & Kevil, C. G. Endothelial dysfunction and diabetes: effects on angiogenesis, vascular remodeling, and wound healing. Int J Vasc Med 2012, 918267 (2012).

  94. 94.

    Leopold, J. A. Cellular and molecular mechanisms of arterial stiffness associated with obesity. Hypertension 62, 1003–1004 (2013).

  95. 95.

    Cox, T. R. & Erler, J. T. Remodeling and homeostasis of the extracellular matrix: implications for fibrotic diseases and cancer. Dis Model Mech 4, 165–178 (2011).

  96. 96.

    Theodossis, T. A., Thrasivoulou, C., Ekwobi, C. & Becker, D. L. Second Harmonic Generation Confocal Microscopy of Collagen Type I from Rat Tendon Cryosections. Biophys J. 91, 4665–4677 (2006).

  97. 97.

    Bhowmick, N. A., Neilson, E. G. & Moses, H. L. Stromal fibroblasts in cancer initiation and progression. Nature 432, 332–337 (2004).

  98. 98.

    Pradeep, C. R. et al. Modeling ductal carcinoma in situ: a HER2-Notch3 collaboration enables luminal filling. Oncogene 31, 907–917 (2012).

  99. 99.

    Pradeep, C. R. et al. Modeling invasive breast cancer: growth factors propel progression of HER2-positive premalignant lesions. Oncogene 31, 3569–3583 (2012).

  100. 100.

    Leung, C. T. & Brugge, J. S. Outgrowth of single oncogene-expressing cells from suppressive epithelial environments. Nature 482, 410–413 (2012).

  101. 101.

    Korkaya, H., Paulson, A., Iovino, F. & Wicha, M. S. HER2 regulates the mammary stem/progenitor cell population driving tumorigenesis and invasion. Oncogene 27, 6120–6130 (2008).

  102. 102.

    Park, K., Han, S., Kim, H. J., Kim, J. & Shin, E. HER2 status in pure ductal carcinoma in situ and in the intraductal and invasive components of invasive ductal carcinoma determined by fluorescence in situ hybridization and immunohistochemistry. Histopathology. 48, 702–707 (2006).

  103. 103.

    Somerville, J. E., Clarke, L. A. & Biggart, J. D. c-erbB-2 overexpression and histological type of in situ and invasive breast carcinoma. J Clin Pathol. 45, 16–20 (1992).

  104. 104.

    Bartkova, J., Barnes, D. M., Millis, R. R. & Gullick, W. J. Immunohistochemical demonstration of c-erbB-2 protein in mammary ductal carcinoma in situ. Hum Pathol. 21, 1164–1167 (1990).

  105. 105.

    Trost, T. M. et al. Premature senescence is a primary fail-safe mechanism of ERBB2-driven tumorigenesis in breast carcinoma cells. Cancer Res. 65, 840–849 (2005).

  106. 106.

    Zacarias-Fluck, M. F. et al. Effect of cellular senescence on the growth of HER2-positive breast cancers. J Natl Cancer Inst 107, djv020 (2015).

  107. 107.

    Sherman, M. Y., Meng, L., Stampfer, M., Gabai, V. L. & Yaglom, J. A. Oncogenes induce senescence with incomplete growth arrest and suppress the DNA damage response in immortalized cells. Aging Cell. 10, 949–961 (2011).

  108. 108.

    Flores, J. M., Martín-Caballero, J. & García-Fernández, R. A. p21 and p27 a shared senescence history. Cell Cycle 13, 1655–1656 (2014).

  109. 109.

    Capparelli, C. et al. CDK inhibitors (p16/p19/p21) induce senescence and autophagy in cancer-associated fibroblasts, “fueling” tumor growth via paracrine interactions, without an increase in neo-angiogenesis. Cell Cycle 11, 3599–3610 (2012).

  110. 110.

    Isola, J. et al. Genetic alterations in ERBB2-amplified breast carcinomas. Clin Cancer Res 5, 4140–4145 (1999).

  111. 111.

    Ithimakin, S. et al. HER2 drives luminal breast cancer stem cells in the absence of HER2 amplification: implications for efficacy of adjuvant trastuzumab. Cancer Res. 73, 1635–1646 (2013).

  112. 112.

    Arendt, L. M. et al. Anatomical localization of progenitor cells in human breast tissue reveals enrichment of uncommitted cells within immature lobules. Breast Cancer Res. 166, 453 (2014).

  113. 113.

    O’Connor, M. D. et al. Alkaline phosphatase-positive colony formation is a sensitive, specific, and quantitative indicator of undifferentiated human embryonic stem cells. Stem Cells 26, 1109–1116 (2008).

  114. 114.

    Oakes, S. R., Gallego-Ortega, D. & Ormandy, C. J. The mammary cellular hierarchy and breast cancer. Cell Mol Life Sci 71, 4301–4324 (2014).

  115. 115.

    Ricardo, S. et al. Breast cancer stem cell markers CD44, CD24 and ALDH1: expression distribution within intrinsic molecular subtype. J Clin Pathol 64, 937–946 (2011).

  116. 116.

    Wright, M. H. et al. Brca1 breast tumors contain distinct CD44+/CD24− and CD133+ cells with cancer stem cell characteristics. Breast Cancer Res. 10, R10 (2008).

  117. 117.

    Morel, A. P. et al. A stemness-related ZEB1-MSRB3 axis governs cellular pliancy and breast cancer genome stability. Nat Med 23, 568–578 (2017).

  118. 118.

    Deng, X. et al. CD24 Expression and differential resistance to chemotherapy in triple-negative breast cancer. Oncotarget 8, 38294–38308 (2017).

  119. 119.

    Lombardo, Y., de Giorgio, A., Coombes, C. R., Stebbing, J. & Castellano, L. Mammosphere formation assay from human breast cancer tissues and cell lines. J Vis Exp, 52671 (2015).

  120. 120.

    Shaw, F. L. et al. A detailed mammosphere assay protocol for the quantification of breast stem cell activity. J. Mammary Gland Biol. Neoplasia 17, 111–117 (2012).

  121. 121.

    Morata-Tarifa, C. et al. Low adherent cancer cell subpopulations are enriched in tumorigenic and metastatic epithelial-to-mesenchymal transition-induced cancer stem-like cells. Sci Rep. 6, 18772 (2016).

  122. 122.

    Dhawan, A. et al. Mathematical modelling of phenotypic plasticity and conversion to a stem-cell state under hypoxia. Scientific Reports 6, 18074 (2016).

  123. 123.

    Cioce, M. et al. Mammosphere-forming cells from breast cancer cell lines as a tool for the identification of CSC-like- and early progenitor-targeting drugs. Cell Cycle 9, 2878–2887 (2010).

  124. 124.

    Wang, R. et al. Comparison of mammosphere formation from breast cancer cell lines and primary breast tumors. J Thorac Dis. 6, 829–837 (2014).

  125. 125.

    Stingl, J., Eaves, C. J., Zandieh, I. & Emerman, J. T. Characterization of bipotent mammary epithelial progenitor cells in normal adult human breast tissue. Breast Cancer Res Treat. 67, 93–109 (2001).

  126. 126.

    Rota, L. M., Lazzarino, D. A., Ziegler, A. N., LeRoith, D. & Wood, T. L. Determining mammosphere-forming potential: application of the limiting dilution analysis. J Mammary Gland Biol Neoplasia 17, 119–123 (2012).

  127. 127.

    Rappa, G. & Lorico, A. Phenotypic characterization of mammosphere-forming cells from the human MA-11 breast carcinoma cell line. Exp Cell Res 16, 1576–1586 (2010).

  128. 128.

    Ghebeh, H. et al. Profiling of normal and malignant breast tissue show CD44high/CD24low phenotype as a predominant stem/progenitor marker when used in combination with Ep-CAM/CD49f markers. BMC Cancer 13, 289 (2013).

  129. 129.

    Smart, C. E. et al. In vitro analysis of breast cancer cell line tumourspheres and primary human breast epithelia mammospheres demonstrates inter- and intrasphere heterogeneity. PLoS One 8, e64388 (2013).

  130. 130.

    Cardnell, R. J. et al. Sepiapterin ameliorates chemically induced murine colitis and azoxymethane-induced colon cancer. J Pharmacol Exp Ther. 347, 117–125 (2013).

  131. 131.

    Cho, Y. R. et al. Sepiapterin inhibits cell proliferation and migration of ovarian cancer cells via down-regulation of p70S6K-dependent VEGFR-2 expression. Oncol. Rep. 26, 861–867 (2011).

  132. 132.

    Rabender, C. S. et al. Sepiapterin Enhances Tumor Radio- and Chemosensitivities by Promoting Vascular Normalization. J Pharmacol Exp Ther 365, 536–543 (2018).

  133. 133.

    Baumgardt, S. L. et al. Chronic Co-Administration of Sepiapterin and L-Citrulline Ameliorates Diabetic Cardiomyopathy and Myocardial Ischemia/Reperfusion Injury in Obese Type 2 Diabetic Mice. Circ Hear Fail 9, e002424 (2016).

  134. 134.

    Pannirselvam, M., Simon, V., Verma, S., Anderson, T. & Triggle, C. R. Chronic oral supplementation with sepiapterin prevents endothelial dysfunction and oxidative stress in small mesenteric arteries from diabetic (db/db) mice. Br J Pharmacol 140, 701–706 (2003).

  135. 135.

    Xian, W., Schwertfeger, K. L., Vargo-Gogola, T. & Rosen, J. M. Pleiotropic effects of FGFR1 on cell proliferation, survival, and migration in a 3D mammary epithelial cell model. J Cell Biol 171, 663–673 (2005).

  136. 136.

    Huerta, S., Chilka, S. & Bonavida, B. Nitric oxide donors: novel cancer therapeutics (review). Int J Oncol 33, 909–927 (2008).

  137. 137.

    Rabender, C. S. The Role of Nitric Oxide Dysregulation in Tumor Maintenance Ph.D. thesis, Virginia Commonwealth University (2013).

  138. 138.

    Malinski, T. & Taha, Z. Nitric oxide release from a single cell measured in situ by a porphyrinic-based microsensor. Nature 358, 676–678 (1992).

  139. 139.

    Beckman, J. S. & Koppenol, W. H. Nitric oxide, superoxide, and peroxynitrite: the good, the bad, and ugly. Am J Physiol. 271, C1424–1437 (1996).

  140. 140.

    Cereser, B. et al. Analysis of clonal expansions through the normal and premalignant human breast epithelium reveals the presence of luminal stem cells. J. Pathol. 244, 61–70 (2018).

  141. 141.

    Pershing, N. L., Yang, C. F. J., Xu, M. & Counter, C. M. Treatment with the nitric oxide synthase inhibitor L-NAME provides a survival advantage in a mouse model of Kras mutation-positive, non-small cell lung cancer. Oncotarget 7, 42385–42392 (2016).

  142. 142.

    Yu, L. B., Dong, X. S., Sun, W. Z., Zhao, D. L. & Yang, Y. Effect of a nitric oxide synthase inhibitor NG-nitro-L-arginine methyl ester on invasion of human colorectal cancer cell line SL-174T. World J Gastroenterol 11, 6385 (2005).

  143. 143.

    Caneba, C. A. et al. Nitric oxide is a positive regulator of the Warburg effect in ovarian cancer cells. Cell Death Dis 5, e1302 (2014).

  144. 144.

    Vyas-Read, S., Shaul, P. W., Yuhanna, I. S. & Willis, B. C. Nitric oxide attenuates epithelial-mesenchymal transition in alveolar epithelial cells. Am J Physiol Lung Cell Mol Physiol. 293, L212–221 (2007).

  145. 145.

    Le, X., Wei, D., Huang, S., Lancaster, J. R. & Xie, K. Nitric oxide synthase II suppresses the growth and metastasis of human cancer regardless of its up-regulation of protumor factors. Proceedings of the National Academy of Sciences of the United States of America 102, 8758–8763 (2005).

  146. 146.

    Hirakawa, M., Oike, M., Masuda, K. & Ito, Y. Tumor Cell Apoptosis by Irradiation-induced Nitric Oxide Production in Vascular Endothelium. Cancer Research 62, 1450–1457 (2002).

  147. 147.

    Reis, O. T. G., Raini, J. C., Coradi, S. T. & Constantino, D. H. J. Effect of L-Arginine and L-NAME treatments on polymorphonuclear leukocytes and mononuclear cells influx during tumor growth. Acta Cirurgica Brasileira 24, 107–111 (2009).

  148. 148.

    Granados-Principal, S. et al. Inhibition of iNOS as a novel effective targeted therapy against triple-negative breast cancer. Breast Cancer Research 17, 25, https://doi.org/10.1186/s13058-015-0527-x (2015).

  149. 149.

    Wang, B. et al. Intact nitric oxide synthase II gene is required for interferon-beta-mediated suppression of growth and metastasis of pancreatic adenocarcinoma. Cancer Res. 61, 71–75 (2001).

  150. 150.

    Shatanawi, A. & Qasrawi, H. Arginase Inhibition Suppresses Breast Cancer Cell Proliferation. The FASEB Journal 31, lb529–lb529, https://doi.org/10.1096/fasebj.31.1_supplement.lb529 (2017).

  151. 151.

    Moncada, S., Palmer, R. M. & Higgs, E. A. Nitric oxide: physiology, pathophysiology, and pharmacology. Pharmacol Rev 43, 109–142 (1991).

  152. 152.

    Pickup, M. W., Novitskiy, S. & Moses, H. L. The roles of TGFβ in the tumour microenvironment. Nat Rev cancer 13, 788–799 (2013).

  153. 153.

    Daoud, S. A., Ismail, W. M., Abdelhamid, M. S., Nabil, T. M. & Daoud, S. A. Possible Prognostic Role of HER2/Neu in Ductal Carcinoma In Situ and Atypical Ductal Proliferative Lesions of the Breast. Asian Pac J. Cancer Prev. 17, 3733–3736 (2016).

  154. 154.

    ten Dijke, P. & Arthur, H. M. Extracellular control of TGF[beta] signalling in vascular development and disease. Nat Rev Mol Cell Biol 8, 857–869 (2007).

  155. 155.

    Harari, D. & Yarden, Y. Molecular mechanisms underlying ErbB2/HER2 action in breast cancer. Oncogene 19, 6102–6114 (2000).

  156. 156.

    Liu, Q. et al. A novel HER2 gene body enhancer contributes to HER2 expression. Oncogene 37, 687 (2017).

  157. 157.

    Scott, G. K., Xu, M. C., Kirk, F., Benz, L. & Transcriptional, C. C. repression of ErbB2 by histone deacetylase inhibitors detected by a genomically integrated ErbB2 promoter-reporting cell screen. Mol Cancer Ther. 1, 385–392 (2002).

  158. 158.

    Scott, G. K. et al. Destabilization of ERBB2 transcripts by targeting 3′ untranslated region messenger RNA associated HuR and histone deacetylase-6. Mol Cancer Res. 6, 1250–1258 (2008).

  159. 159.

    Peng, X. et al. DB. Heat shock protein 90 stabilization of ErbB2 expression is disrupted by ATP depletion in myocytes. J Biol Chem 280, 13148–13145 (2005).

  160. 160.

    Koo, J. S., Jung, W. & Yang, W. I. HER-2 protein overexpressing breast cancer without gene amplification shows higher hormone receptor expression than HER-2 protein overexpressing breast cancer with gene amplification. Int J Surg Pathol 19, 425–432 (2011).

  161. 161.

    Kuo, S. J. et al. Comparison of immunohistochemical and fluorescence in situ hybridization assessment for HER-2/neu status in Taiwanese breast cancer patients. Taiwan J Obstet Gynecol. 46, 146–151 (2007).

  162. 162.

    Lee, T. Y. et al. dbSNO: a database of cysteine S-nitrosylation. Bioinformatics 28, 2293–2295 (2012).

  163. 163.

    Sonveaux, P., Jordan, B. F., Gallez, B. & Feron, O. Nitric oxide delivery to cancer: why and how? Eur J Cancer 45, 1352–1369 (2009).

  164. 164.

    Heilman, B. & Mascharak, P. K. Light-triggered nitric oxide delivery to malignant sites and infection. Philos Trans A Math Phys Eng Sci. 371, 20120368 (2013).

  165. 165.

    Eroy-Reveles, A. A. & Mascharak, P. K. Nitric oxide-donating materials and their potential in pharmacological applications for site-specific nitric oxide delivery. Future Med Chem 1, 1497–1507 (2009).

  166. 166.

    Laakkonen, P. & Vuorinen, K. Homing peptides as targeted delivery vehicles. Integr Biol 2, 326–337 (2010).

  167. 167.

    Pigott, B., Bartus, K. & Garthwaite, J. On the selectivity of neuronal NOS inhibitors. Br J Pharmacol 168, 1255–1265 (2013).

  168. 168.

    Plante, l, Stewart, M. K. & Laird, D. W. Evaluation of mammary gland development and function in mouse models. J Vis Exp 53, 2828 (2011).

  169. 169.

    Grivel, J. C. & Margolis, L. Use of human tissue explants to study human infectious agents. Nat Protoc. 4, 256–269 (2009).

  170. 170.

    DeRose, Y. S. et al. Patient-derived models of human breast cancer: protocols for in vitro and in vivo applications in tumor biology and translational medicine. Curr Protoc Pharmacol. Chapter 14, 23 (2013).

  171. 171.

    Lawrenson, K., Grun, B. & Gayther, S. A. Heterotypic three-dimensional in vitro modeling of stromal-epithelial interactions during ovarian cancer initiation and progression. J Vis Exp 28, e4206 (2012).

  172. 172.

    de la Mare, J. A. et al. Assessment of potential anti-cancer stem cell activity of marine algal compounds using an in vitro mammosphere assay. Cancer Cell Int 13, 39 (2013).

  173. 173.

    McCLAY, D. R., Gooding, L. R. & Fransen, M. E. A requirement for trypsin-sensitive cell-surface components for cell-cell interactions of embryonic neural retina cells. J Cell Biol. 75, 56–66 (1977).

  174. 174.

    Lee, S.-Y. et al. FAM83A confers EGFR-TKI resistance in breast cancer cells and in mice. J Clin Invest 122, 3211–3220 PMCID: PMC3428077 (2012).

  175. 175.

    McHugh, M. L. Multiple comparison analysis testing in ANOVA. Biochem Med (Zagreb) 21, 203–209 (2011).

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Acknowledgements

We thank Dr. Hongliu Sun (Department of Pathology, UT), as well as other staffs in the Department of Pathology, UT, for preparation and evaluation of histological specimens; and all the DLAR staffs, especially, Dr. Phillip T. Robinson, Ms. Katherina Goans and Ms. Jeanna Ronau for veterinary care, husbandry, training and technical support for animal studies. This work was supported by the startup fund from University of Toledo Health Science Campus, College of Medicine and Life Sciences, Department of Cancer Biology to S.F.; Ohio Cancer Research Grant (Project #: 5017) to S.F; Medical Research Society (Toledo Foundation) Award to S.F; American Cancer Society Research Scholar Grant (RSG-18-238-01-CSM) to S.F; UT Office of Research URFO Biomedical Research Award to KY; and Fully Honest Corp Research Grant to KY.

Author information

S.F. designed the project and supervised the study. G.R., X.Z., M.B., S.M., A.S., C.F. and K.Y. prepared samples and reagents. G.R., X.Z., M.B., Y.W., A.K. and D.W. conducted experiments and/or acquired/analyzed the data. G.R. and M.B. performed animal experiments. M.B., Y.W., J.L. and S.F. quantified and interpreted the data. S.F., M.B. and J.L. compiled the data and constructed figures. X.Z., Y.W. and J.L. performed experiments for revision. S.F., M.B. and S.M. wrote the manuscript. G.R. and X.Z. provided the information for materials and methods and figure legends. S.F., J.L., M.B., Y.W., S.M., X.Z. and G.R. proofread the manuscript.

Correspondence to Saori Furuta.

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Ren, G., Zheng, X., Bommarito, M. et al. Reduced Basal Nitric Oxide Production Induces Precancerous Mammary Lesions via ERBB2 and TGFβ. Sci Rep 9, 6688 (2019) doi:10.1038/s41598-019-43239-x

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