The mammary gland experiences substantial remodeling and regeneration during development and reproductive life, facilitated by stem cells and progenitors that act in concert with physiological stimuli. While studies have focused on deciphering regenerative cells within the parenchymal epithelium, cell lineages in the stroma that may directly contribute to epithelial biology is unknown. Here we identify, in mouse, the transition of a PDGFRα+ mesenchymal cell population into mammary epithelial progenitors. In addition to being adipocyte progenitors, PDGFRα+ cells make a de novo contribution to luminal and basal epithelia during mammary morphogenesis. In the adult, this mesenchymal lineage primarily generates luminal progenitors within lobuloalveoli during sex hormone exposure or pregnancy. We identify cell migration as a key molecular event that is activated in mesenchymal progenitors in response to epithelium-derived chemoattractant. These findings demonstrate a stromal reservoir of epithelial progenitors and provide insight into cell origins and plasticity during mammary tissue growth.
The mammary parenchyma comprises an inner layer of luminal epithelial cells and an outer basal epithelial lineage1. The luminal lineage can differentiate into lobuloalveolar structures during the female reproductive cycle and become milk-secreting sacs following pregnancy. The basal lineage gives rise to differentiated myoepithelial cells that are contractile and aid in milk expulsion. Early mammary development as well as adult tissue growth and regeneration rely on stem cells and progenitors to generate epithelial lineages upon physiological demand. Research on mammary epithelial precursors has been fueled by therapeutic challenges in breast cancer arising from breast cancer heterogeneity and evidence suggests that mammary stem cells or their progenitors are putative cells of origin in distinct breast cancer subtypes2. Work from several groups3,4,5,6,7,8,9,10,11,12 has yielded knowledge on the existence, characteristics, potency, location, and regulation of mammary stem and progenitor cells within epithelial lineages.
The mammary epithelium is embedded in an adipose-rich stroma that contains haematopoietic, endothelial cells, the extracellular matrix and mesenchymal cells such as fibroblasts and adipocyte precursors. The importance of stromal-epithelial interactions for mammary gland biology and breast cancer has long been appreciated13,14. As early as embryonic development, the mesenchyme is known to induce formation of the mammary epithelial bud13. The greater part of mammary growth and branching that takes place during postnatal life is dependent on an intricate interplay between the hypothalamic-pituitary-ovarian hormone axis and cell-cell communications where diverse stromal elements play a crucial role14. In breast cancer, carcinoma associated fibroblasts in the tumor microenvironment drive tumor growth and metastasis15. A significant stromal influence on early cancer development is also evident in studies where exposure of the stroma alone to carcinogens is sufficient to trigger tumorigenesis within the epithelium16,17. While mammary stem cells and progenitors are recognized precursors for epithelial expansion, our understanding of the impact of stromal niche cells on these cell populations is rather limited18,19. In particular, stromal lineages that directly contribute to the epithelial precursor pool have not been defined.
Adipocytes are abundant in mammary stroma and tissue-ablation studies in mice have inferred the importance of adipocytes in mammary development20,21. In white adipose tissue depots, adipocytes have been shown to arise from resident adipocyte progenitors22,23. Lineage tracing studies have established Platelet Derived Growth Factor Receptor alpha (PDGFRα) as a marker of adipocyte progenitors that can generate de novo functional adipocytes in vivo24,25. PDGFRα is expressed by mesenchymal cell populations and is involved in the development of diverse tissues26,27.In skin epithelia, adipocyte precursor cells are involved in driving the regenerative hair cycle28. The mammary gland is a skin appendage and similar to the hair follicle, it undergoes significant growth and cyclical remodeling in postnatal life29. However, dynamics of adipocyte progenitors during mammary epithelial expansion have been unexplored.
Here, we show that PDGFRα marks mesenchymal adipocyte progenitors that form a distinct stromal layer encasing the parenchymal epithelial lineages of the mouse mammary gland. PDGFRα+ progeny are present in mammary epithelial lineages from early embryonic development and throughout morphogenesis in postnatal life. These stromal progenitors are recruited into the mammary epithelium during early development and in the adult gland upon steroid sex hormone exposure or pregnancy. We find that mesenchymal adipocyte precursors marked by Preadipocyte factor 1 (PREF-1) also transition into adult mammary epithelial cells while mature adipocytes do not. Through combined transplantation and lineage tracing experiments, we demonstrate the mesenchymal-to-epithelial switch of stroma-localized cells during mammary epithelial expansion. PDGFRα+ stromal cells exhibit a robust migratory molecular profile in response to sex hormones in vivo. We observe increased expression levels of Pdgfc, a PDGFRα ligand, in epithelial cells from hormone-stimulated mice, and illustrate chemotactic migration of PDGFRα+ stromal cells following PDGFCC administration. Taken together, this study exposes a PDGFRα+ and PREF-1+ mesenchymal adipogenic cell pool as a source of epithelial descendents in the expanding mammary gland.
PDGFRα marks mesenchymal progenitors in the mammary gland
Given the abundant adipose content in the adult mammary gland, we examined whether PDGFRα can serve as a marker of mammary stromal progenitors. In addition to being scattered throughout the mouse fat pad, PDGFRα+ stromal cells formed a concentrated layer closely surrounding the bilayered mammary epithelium, which comprises inner luminal cells and outer basal cells1 (Fig. 1a). This distribution persisted during the estrous reproductive cycle or following hormonal stimulation (Supplementary Fig. 1a). Despite the striking proximity of PDGFRα+ cells to epithelial structures, co-staining with luminal- and basal-specific cytokeratins showed that PDGFRα does not overlap with epithelial keratins (Fig. 1a). Based on established cell surface marker profiles3,30, stromal (CD49f-EpCAM-), luminal (CD49floEpCAM+) and basal (CD49fhiEpCAM+) cell fractions were purified using fluorescence-activated cell sorting (FACS) and Pdgfrα expression was analyzed by droplet digital PCR (ddPCR) used for detecting low mRNA levels (Fig. 1b). Pdgfrα transcripts were only observed in the stromal fraction, and absent in K14-expressing basal and K18-expressing luminal cells. Mice treated with either vehicle or sex hormones (estrogen, E; estrogen and progesterone, E+P) also showed Pdgfrα mRNA expression exclusively in stromal cells (Supplementary Fig. 1b). Next, flow cytometry of PDGFRα+ cells showed their presence in lineage- cells but not in the lineage+ hematopoietic and endothelial populations (Fig. 1c). Within lineage- cells, PDGFRα+ cells were significantly present in the stromal mesenchymal subset, but not found in epithelial fractions (basal, luminal, or luminal subpopulations segregated by Sca1 that enriches for estrogen and progesterone receptor positive (ER+PR+, Sca1+) versus negative (ER-PR-, Sca1-) cells and progenitors;30,31 Fig. 1d, e). The proportion of PDGFRα+ cells in the stroma increased upon hormone stimulation indicative of their hormone sensitivity (Fig. 1e). FACS-sorted PDGFRα+ cells differentiated into lipid-laden adipocytes in vitro (Fig. 1f), and were enriched for stromal progenitors as seen through their increased colony forming capacity (Fig. 1g–i). These data identify a PDGFRα+ progenitor population that is hormone-sensitive and adipogenic in the mammary stroma.
Progeny of the Pdgfrα+ lineage exists in mammary epithelium
We then investigated the fate of PDGFRα+ stromal progenitors in the mammary gland by crossing PdgfrαCre mice to Rosa26mTmG reporters. The resulting PdgfrαCreR26mTmG lineage tracing mice have indelible eGFP labeling of Pdgfrα+ cells and their progeny after Cre-mediated excision of tdTomato in Pdgfrα-expressing cells (Fig. 2a). In adult PdgfrαCreR26mTmG females, native GFP fluorescence was seen in adipocytes of mammary whole mounts by confocal imaging (Fig. 2b), confirming Pdgfrα+ cells as adipocyte precursors in vivo as previously reported for male adipose tissue depots25. Remarkably, GFP was observed throughout the gland in mammary epithelial structures (Fig. 2b and Supplementary Movie 1). Tissue sections revealed the distribution patterns of PDGFRα+ cells in relation to GFP+ progeny. Specifically, PDGFRα+ cells were dispersed in the fat pad and adjacent to ducts, yet restricted to stroma while GFP+ cells comprised PDGFRα+ stromal cells, adipocytes and epithelial cells (Fig. 2c, d and Supplementary Fig. 2a). GFP+PDGFRα- cells were found in both the basal and luminal epithelial layers, with luminal GFP+ cells being primarily PR- (Supplementary Fig. 2a). FACS enumeration demonstrated that GFP+ progeny was present in epithelial compartments in addition to stroma, and dominated the basal compartment and Sca1- luminal progenitor subset, both of which are generally hormone-receptor negative (Fig. 2e, f and Supplementary Fig. 2b).
Given this unexpected occurrence of PDGFRα+ stromal progeny in epithelia, we performed ddPCR on FACS-purified mammary subsets from Cre+ mice and Cre- controls to measure Pdgfrα expression in our lineage tracing study; Pdgfrα transcript was only detected in stroma (Fig. 2g). We next investigated PDGFRα+ progenitor dynamics during early development, and found that PDGFRα remained stromally-restricted while GFP+ cells in lineage tracing experiments were observed in epithelia of both pubescent (5-week) and prepubescent (2-week) glands through imaging and FACS analyses (Fig. 2h–j and Supplementary Fig. 3a-d). Tracing in the mammary rudiment at embryonic day 18 (E18) and bud as early as E13 showed localization of PDGFRα to the mammary mesenchyme and the presence of GFP progeny in epithelial layers that expressed EpCAM, K14 and K19 (Fig. 2k, l and Supplementary Fig. 3e, f). These in situ and quantitative data pinpointed PDGFRα+ stromal precursors as a previously unrecognized source of mammary epithelial progenitors.
Adipocyte progenitors contribute to mammary epithelia
We next used a series of mouse models to discern the recruitment of mesenchymal stromal lineage cells into the adult mammary epithelium. We first checked endogenous Pdgfrα expression using PdgfrαH2B-eGFP mice that harbor a histone H2B-eGFP fusion reporter controlled by the Pdgfrα promoter (Fig. 3a). In immunostained tissue sections, GFP+ cells were present in the PDGFRα+ stroma but not epithelium (Fig. 3b). Flow cytometry showed a marked H2B-eGFP+ stromal population whereas epithelial cells expressed 1–2 orders of magnitude lower GFP fluorescence intensity (Fig. 3c, d). Pdgfrα analysis by ddPCR in FACS-purified GFP+ stroma versus low intensity GFP+ basal and luminal subsets verified detectable transcripts only in GFP+ stroma (Fig. 3e), indicating that the low epithelial GFP reflects prior Pdgfrα expression in the stromal parental lineage. We employed inducible PdgfrαCreERTR26mTmG mice which have previously been used to trace the adipocyte lineage in white adipose tissue24. Here, Cre-driven eGFP expression is induced following tamoxifen (TAM) administration (Supplementary Fig. 4a), enabling temporal control over cell labeling and fate mapping. In a 3-day short trace, mammary tissue from TAM-treated mice had prominent GFP in PDGFRα+ stromal cells (Fig. 4a–c and Supplementary Fig. 4b, e). Occasional GFP+ PDGFRα- epithelial cells were noted, some of which had finger-like projections in contact with the PDGFRα+ stroma, signifying a transitory state (Supplementary Fig. 4c). Oil-injected Cre+ controls did not show GFP in whole mounts, tissue sections or by flow cytometry, thus precluding possible leaky Cre expression (Supplementary Fig. 4d, e).
Ovarian sex hormones, especially progesterone, are well known to activate mammary stem cells and progenitors in the adult gland propelling the growth of milk-secreting lobuloalveoli during the mouse and human reproductive cycle as well as pregnancy1,10,32,33. Thus, we incorporated sex hormone treatment or pregnancy in a ~3-week trace following TAM (Fig. 4d–i). After hormone exposure, GFP+ cells contributed to epithelial expansion in lobuloalveolar structures, remained PDGFRα-, were largely PR- and epithelial EpCAM+ although Keratin low, and accumulated mainly in luminal progenitor subsets (Fig. 4e, f and Supplementary Fig. 5a, b and Supplementary Movie 2, 3). Of note, PDGFRα+ GFP+ cells often exhibited long cellular processes, and in certain instances formed long stretches contiguous with PDGFRα- GFP+ cells in the epithelium (Fig. 4e and Supplementary Movie 3). Tracing in mid-pregnancy (Fig. 4g), GFP-labeled cells similarly demonstrated their expansion within lobuloalveoli, again mostly in the luminal compartment (Fig. 4h, i and Supplementary Fig. 5c, d). We also found that induction of lineage tracing during early development in mice 2 weeks old or less resulted in a vast proportion of GFP+ progeny in luminal as well as basal subsets when analyzed in older mice, indicating significant contribution of PDGFRα+ cells to early formation of the mammary gland (Fig. 5a, b and Supplementary Fig. 6).
Preadipocyte factor-1 (Pref-1 or Dlk1) has been shown to specifically mark mesenchymal adipocyte precursors essential during embryonic white adipose tissue development and adult adipose tissue expansion34,35. To ascertain the contribution of mesenchymal adipocyte precursors to the mammary epithelium, we selected doxycyline (DOX)-inducible Pref-1-rtTA TRE-Cre R26mTmG mice as an independent lineage tracing model (Fig. 4j). In a short 3-day trace following DOX administration in adult mice, GFP-labeled cells were present in mammary stroma surrounding ducts where some overlapped with PDGFRα expression (Supplementary Fig. 7a). Upon longer-tracing involving hormone-stimulated growth of the mammary gland, GFP+ cells were observed within mammary lobuloalveoli and epithelial subsets (Fig. 4k, l and Supplementary Fig. 7b, c), similar to PdgfrαCreERTR26mTmG mice. To determine whether mature adipocytes have the capacity to generate mammary epithelial cells, we TAM-induced adult AdiponectinCreERTR26mTmG mice which have been shown to effectively label mature adipocytes36 (Fig. 4m). Tracing cell fate at mid-pregnancy showed GFP-labeled adipocytes without any epithelial progeny (Fig. 4n and Supplementary Fig. 7d, e). GFP+ adipocytes were also negative for PDGFRα expression (Fig. 4n), as reported previously25 . Together, these data show that mesenchymal adipocyte precursors but not mature adipocytes within the mammary stroma give rise to epithelial descendents which expand during hormone-dependent growth of the adult mammary gland.
Tracing-in-transplants illustrate stromal-to-epithelial transition
We then designed a lineage ‘tracing-in-transplant’ assay (Fig. 6a) to delineate whether mesenchymal cells from a stromal lineage tracing fat pad can indeed contribute to epithelium derived from a non-lineage tracing mouse. FACS-purified, non-fluorescent wild-type mammary epithelial cells were transplanted into inguinal epithelium-divested mammary fat pads of PdgfrαCreERTR26mTmG recipients; care was taken to sever the connection between the fourth and fifth mammary glands to ensure complete clearing of the fourth mammary fat pad. Recipients received TAM 8-weeks after transplant, and then were hormone-stimulated or left untreated. In all transplants, wild type outgrowths were readily visible in tissue sections as nuclear DAPI+ and tdTomato- in contrast to the endogenous DAPI+ tdTomato+ lineage tracing fat pad (Fig. 6b). Notably, sex hormone stimulation following TAM induction generated wild-type outgrowths in all transplanted fat pads that contained GFP+ progeny from the stroma that now contributed to mammary epithelial structures, lost their mesenchymal PDGFRα expression, and instead expressed the epithelial marker EpCAM (Fig. 6b and Supplementary Movie 4). GFP+EpCAM+ epithelial cells also existed as clusters, indicating expansion of epithelial progenitors derived from stromal precursors. In mice untreated with hormones, GFP-labeled cells were only detectable in the stroma (Fig. 6b), indicating that the transplantation technique per se did not elicit a stromal to epithelial lineage switch. Furthermore, when wild type epithelial cells were transplanted into mature adipocyte lineage tracing fat pads of AdiponectinCreERTR26mTmG mice that were subsequently TAM induced and hormone treated, GFP-labeled adipocytes in the stroma did not contribute to epithelia (Fig. 6c, d), showing that sex hormones do not mediate artificial epithelial recruitment of otherwise committed stromal lineages. These series of transplantation experiments unequivocally demonstrate the transition of a mesenchymal niche population into mammary epithelial progenitors.
Adipocyte progenitors exhibit a migratory phenotype
To define molecular features of adipocyte progenitors and their epithelial progeny, we performed RNA-seq on FACS-purified GFP+ and tdTomato+ stromal and luminal populations from untreated (n = 4) and hormone stimulated (n = 3) adult PdgfrαCreR26mTmG mice (Fig. 7a). The mRNA abundance of known lineage markers confirmed a mesenchymal phenotype for the stromal subsets (e.g. Vim, S100a4, Procr, as well as adipocyte precursor markers Pdgfra, Pref-1 (Dlk1), Pparg) while the luminal fractions showed high levels of epithelial markers (e.g. Krt8, K18, K19, Epcam, Itga6 along with basal Krt14; Fig. 7b). GFP+ luminal cells had higher levels of epithelial progenitor genes such as Elf5, Kit, Notch1 and Aldh1a3 and lower levels of estrogen (Esr1) and progesterone (Pgr) receptors, thus signifying enrichment of progenitor features within the GFP+ epithelial progeny. Previous studies have assigned a CD29+CD34+Sca1+ profile to adipocyte progenitors23,24. CD29 and Sca1 are also used in the mammary gland field to distinguish epithelial subpopulations, although we noted Itgb1 (CD29) to be higher in stromal subsets, and Ly6a (Sca1) and Cd34 to be elevated in the GFP+ stromal subpopulation (Fig. 7c), confirming their adipocyte precursor phenotype. Alx4, a stromally restricted homeodomain factor essential for mammary morphogenesis37, was also higher in the GFP+ adipocyte progenitor population that expressed Pdgfrα, where Alx4 increased in response to hormones. These expression profiles affirmed the distinct nature of mesenchymal and epithelial subpopulations purified for our molecular analyses.
Transcriptome comparison of GFP+vs. tdTomato+ populations from all stromal specimens identified 7555 statistically significant differentially expressed genes (DEGs; FDR < 0.01). When the top 20% most variable genes were examined by unsupervised hierarchical clustering, stromal GFP+ and tdTomato+ subsets clustered into discrete groups (Fig. 7d). GFP+ stromal cells were observed to have more similar transcriptomes to luminal cells than to tdTomato+ stromal cells following distance-analysis of DEGs between GFP+ and tdTomato+ subpopulations within stromal and luminal lineages (Supplementary Fig. 8a, b). KEGG pathway analysis of DEGs between GFP+ and tdTomato+ stromal subsets indicated enrichment in pathways that govern Focal adhesion, ECM-receptor interaction, Actin cytoskeleton, Lysosomes and PI3K-Akt signaling (Fig. 7e). Exposure to hormones augmented pathways in cancer, as well as those implicated in cell migration such as Focal Adhesion, Endocytosis and the Phosphatidylinositol System38,39,40. We also noted a decrease in Adherens junction. Interestingly, PDGFRα and its downstream PI3K pathway are involved in directed cell migration26. These analyses inferred a cell migration program is heightened within stromal progenitors following their activation.
We postulated that PDGFRα ligands expressed by epithelial cells in response to hormones could serve as chemotactic stimuli for stromal cell migration. Interrogation of RNA-seq data for known PDGFR ligands revealed that Pdgfa, Pdgfb and Pdgfc were expressed by epithelial cells while Pdgfd was mostly present in stroma (Fig. 7f). Upon hormone exposure, especially in response to both estrogen and progesterone, Pdgfc was most significantly elevated in luminal and basal epithelial subsets, as seen by qRT-PCR of FACS-purified stromal and epithelial fractions (Fig. 7g). In co-cultures of FACS-sorted GFP+ stromal cells from PdgfrαCreR26mTmG mice with Cre- tdTomato+ mammary epithelial organoids, addition of PDGFCC was seen to stimulate GFP+ stromal cell movements into epithelial organoids as monitored through live time-lapse imaging (Fig. 7h and Supplementary Movie 5, 6). To determine whether PDGFCC stimulates chemotactic migration of GFP+ stromal cells that generate epithelial progeny, the FACS-sorted cells above were plated onto transwell inserts in a Boyden chamber assay, and cell migration measured in response to recombinant PDGFCC (Fig. 7i). This PDGFRα ligand significantly increased stromal cell migration compared to control (Fig. 7j, k). Thus, adipocyte precursor cells in the mammary stroma are likely activated in response to expansion cues through a hormone-PDGFCC-PDGFRα axis to disengage from their adipogenic program, migrate into the epithelium and adopt an epithelial cell fate (Fig. 8).
Our findings show plasticity of mesenchymal cells within stroma wherein adipocyte progenitors undergo cell fate transformation into epithelial progenitors during mammary parenchymal growth. Previous work has documented a potential of in vitro expanded adipose derived stromal cells to reprogram into different cell types primarily in in vitro settings41,42,43, where the stromal cells comprise of a heterogeneous population derived from the adipose stromal-vascular fraction and lack specificity for adipocyte progenitors. A previous report described a capacity of mature adipocytes to transdifferentiate into mammary secretory epithelial cells during pregnancy, and of secretory epithelial cells to revert to adipocytes during involution44. In contrast, we did not observe adipocyte to epithelial transformation with the mature adipocyte-specific Adiponectin-CreERT line. Interestingly, a recent study found that metastasis formation could be suppressed when invasive breast cancer cells that have undergone an epithelial to mesenchymal transition are induced to become adipocytes45, underscoring the highly plastic nature of mesenchymal cells.
Adipose tissue also plays an important role in energy homeostasis and excess adiposity is linked to increased risk of epithelial cancers including breast cancer46,47. In addition to adipocyte hypertrophy, adipose tissue accumulation is a result of adipocyte hyperplasia that is attributed to a recruitment of adipocyte progenitors48. Several mechanisms have been proposed to underlie the pathophysiological link between adiposity and cancer, largely involving adipokines and insulin49. Since most adiposity-related cancers occur in organs that are embedded in adipose tissue such as the breast, the roles of local adipose tissue resident cells including their progenitors in cancer development and progression are also of great interest50. Thus, studying adipocyte progenitor biology in the normal breast is essential for understanding its potential involvement in breast cancer.
In this study, we add a fundamental layer to the mammary epithelial hierarchy where stromal cells that possess an adipocyte progenitor identity exit their mesenchymal niche to populate the epithelial niche and actively generate cells within progenitor-enriched compartments, culminating in epithelial expansion during mammary growth. Postnatal mammary growth and remodeling are tightly controlled by hormones1 and we observed stromal cell recruitment and increased presence of their progeny in the epithelium during hormone-driven stages. Exogenous sex hormone supplementation in many of our experiments induced a consistent growth stimulus that mirrors in part the hormone milieu found during the physiological progesterone-dominant reproductive phase and pregnancy, resulting in lobuloalveolar formation. Further, we report PDGFRα+ mesenchymal cell contribution to the mammary epithelial network during early development and pregnancy. We provide evidence that steroid sex hormones induce PDGF signals in the epithelium which act to mobilize PDGFRα+ mesenchymal niche cells, stimulating their migration in a chemotactic manner. In the human breast, a distinct fibroblast lineage which has adipogenic capacity and supports the growth of luminal epithelial progenitors has been reported that accumulates around terminal ductal lobular units (TDLUs)51. It is possible that this fibroblast lineage has properties similar to the mesenchymal population that we describe here given that we see a prominent contribution of mesenchymal adipocyte progenitors to mouse mammary lobuloalveoli which are analogous structures to human TDLUs52. We show that this stromal lineage preferentially contributes to luminal progenitors in the adult mammary gland, a population implicated in aggressive BRCA1-mutated breast cancer53,54. Increased lifetime hormone exposure is a well known risk factor for breast cancer55 and in combination with increased adiposity or an aberrant metabolic state, hormone-responsive adipocyte precursors may contribute to malignant transformation in breast epithelia. In light of the global health crisis that is underway with increasing rates of adiposity, diabetes and associated increased risk of several cancers56, deconstructing adipocyte progenitor biology within tissue niches is pivotal not only for understanding its impact on adipose tissue mass, but also for elucidating the link between adiposity and cancer.
PdgfrαCre (Stock# 013148), PdgfrαCreERT (Stock# 018280), Rosa26mTmG (Stock# 007676), PdgfrαH2B-eGFP (Stock# 007669), AdiponectinCreERT (Stock# 024671) mice were obtained from the Jackson Laboratory. C57BL/6 mice were purchased from Charles River Laboratories. Pref-1-rtTA TRE-Cre Rosa26mTmG mice were provided by Dr. Hei Sook Sul (UC Berkeley). All mice were on the C57BL/6 background and cared for according to the Canadian Council for Animal Care guidelines under protocols approved by the Animal Care Committee of the Princess Margaret Cancer Centre, Toronto, Ontario.
Treatments and lineage tracing
Mice were randomly assigned to groups that either received hormone treatment or were left untreated. Adult wild-type female mice (10–13 weeks old) were treated with 17β-estradiol (E, 0.14 mg) or 17β-estradiol + progesterone (E+P, 0.14 mg E+ 14 mg P) using 14-day slow release pellets (Innovative Research of America) implanted subcutaneously. Hormone treatments were performed in intact mice unless otherwise indicated in the figure legend. Lineage tracing in the PdgfrαCreR26mTmG constitutive model was performed in adult (10–12 week old; comparable estrous stage), pubescent (5 week old), prepubescent (2 week old) female mice and in E18, E13 female embryos. Mice were randomly taken from different litters. For inducible lineage tracing in PdgfrαCreERTR26mTmG and AdiponectinCreERTR26mTmG adult (10 week old) mice, a single intraperitoneal injection of 1.25 mg of 4-hyroxytamoxifen (TAM; Sigma) diluted in sunflower seed oil per 25 g body weight was administered to induce Cre-mediated recombination and GFP labeling. Lineage tracing in PdgfrαCreERTR26mTmG mice less than or equal to 2 weeks of age was induced with 0.5 mg of TAM. Lineage tracing in adult Pref-1-rtTA TRE-Cre Rosa26mTmG mice was induced with a single intraperitoneal injection of 2 mg doxycycline (Sigma) in sterile PBS.
Mammary cell preparation and flow cytometry
Freshly dissected mammary glands from individual mice were digested for 2.5 h at 37 °C in DMEM: F12 with 750 U ml−1 collagenase and 250 U ml−1 hyaluronidase. Digested tissue was vortexed, incubated in NH4Cl red blood cell lysis solution, dissociated in 0.25% trypsin for 2 min and 5mg ml−1 dispase with 0.1mg ml−1 DNaseI for 2 min, prior to filtering through a 40μm mesh to obtain single cells. All reagents were from STEMCELL Technologies. Cells were then labeled with fluorochrome (Pe-Cy7)-conjugated antibodies to CD31 (Ebioscience, Cat.# 25–0311, 1:500), Ter119 (Ebioscience, Cat.# 25–5921, 1:200) and CD45 (Ebioscience; Cat.# 25–0451, 1:1000) for endothelial, erythrocyte and hematopoietic cell exclusion respectively. For segregating mammary epithelial and stromal subpopulations, antibodies used are as follows: anti-CD49f-FITC (BD Pharmingen, Cat.# 555735, 1:50) or anti-CD49f-APC (R&D, Cat.# FAB13501A, 1:50), anti-EpCAM-AF647 (Biolegend, Cat.# 118211, 1:200) or anti-EpCAM-APC/Cy7, Cat.# 118217, 1:200), anti-Sca1-APC/Cy7 (Biolegend, Cat.# 108125, 1:500) or anti-Sca1-Pacific Blue (Biolegend, Cat.# 108119, 1:500) and anti-CD140 (PDGFRα)-PE (Biolegend, Cat.# 135905, 1:200). Dead cells were excluded with propidium iodide staining (PI, Sigma). Flow cytometry analysis was done using FACSCantoII (BD) and FlowJo software (Tree Star, Inc.). Cell sorting was performed on a FACSAria (BD) and the purity of sorted populations was routinely >96%.
Colony forming cell assay and adipocyte differentiation
Stromal mammary subpopulations were FACS-sorted and plated with irradiated NIH 3T3 fibroblasts in DMEM:F12 medium containing 10% FBS (GIBCO), insulin (Life Technologies), EGF (STEMCELL Technologies), cholera toxin (Sigma), adenine (Sigma), hydrocortisone (STEMCELL Technologies), Rock inhibitor (Reagents Direct) and cultured in 5% oxygen conditions as done previously for mammary epithelial cells11. Colonies were scored after 10 days. To induce adipocyte differentiation, the FACS-purified adipocyte progenitor subset was cultured in DMEM supplemented with 10% FBS (GIBCO) and 10 ng/ml bFGF (STEMCELL Technologies), as previously described23. Cells were grown to confluence and held at confluence for 2 days without media change following which a differentiation cocktail containing insulin, dexamethasone and IBMX was added in fresh media without bFGF for 3 days. Cells were then maintained in DMEM with 10% FBS for another 3 days, and subsequently fixed with 2% formaldehyde and 0.2% glutaraldehyde in PBS for 15 min. Cultures were rinsed carefully in PBS, water and 60% isopropanol prior to staining with oil red O (0.7% in 60% isopropanol) for 20 min at room temperature after which they were rinsed with 60% isopropanol and water.
Tissue processing and immunostaining
Dissected mammary glands were fixed for 2 h in 4% paraformaldehyde at room temperature, washed three times with PBS and immersed in 30% sucrose in PBS overnight at 4 °C, after which they were embedded in OCT, stored at −80 and cryosectioned at 5–15μm thickness for immunofluorescence. Frozen sections were incubated in blocking buffer (5% normal donkey serum/1% BSA/0.2% Triton in PBS) for 1 h at room temperature followed by primary antibodies diluted in blocking buffer without Triton overnight at 4 °C. Sections were rinsed and incubated with secondary antibodies for 1 h at room temperature, rinsed again and mounted using ProLong Gold Anti-fade reagent with DAPI. For immunohistochemistry, 4% paraformaldehyde-fixed paraffin-embedded tissue sections were de-paraffinized in xylene, gradually rehydrated in descending concentrations of ethanol, and antigen retrieval performed in Borg Decloaker solution (pH 9) for 5 min at 125 °C using a Decloaking chamber (Biocare Medical). After rinsing in PBS, endogenous peroxidase, avidin and biotin blocking buffers were applied, followed by 5% horse serum block in PBS. Sections were incubated overnight in primary antibody at 4 °C, washed the next day in PBS and incubated with biotinylated horse anti-goat secondary (Vector Labs, Cat.# BA9500, 1:1000) for 1 h at room temperature, followed by Vectastain Elite ABC peroxidase, AEC substrate and counterstained with Mayer’s hematoxylin. Primary antibodies used are as follows: anti-PDGFRα (R&D systems, Cat.# AF1062, 1:200), anti-K8 (LifeSpan Biosciences, Cat.# LS-B12422, 1:200), anti-K14 (Biolegend, Cat.# 906001, 1:400 or Cat.# 905301, 1:1000), anti-K19 (Santa Cruz, Cat.# sc-33111, 1:100), anti-GFP (Abcam, Cat.# ab13970, 1:4,000), anti-tdTomato (Clontech, Cat.# 632496, 1:500), anti-PR (Santa Cruz, Cat.# sc-7208, 1:200) and anti-EpCAM (abcam, Cat.# ab71916, 1:100). Secondary antibodies used are as follows: anti-goat, anti-rabbit, anti-chicken conjugated to AlexaFluor 647, AlexaFluor Cy3, AlexaFluor 488 or Dylight 405 (Jackson ImmunoResearch, 1:300).
Confocal microscopy image acquisition
Freshly dissected and unprocessed mammary glands were placed between a slide and coverslip to image as whole mounts on a Zeiss LSM710 confocal microscope using 20 × /1.0NA (water) and C-Apo 63 × /1.4NA (oil) objectives. Fat was left intact to capture adipocytes. Z-stacks were acquired at 1024 × 1024 optical section resolution. Tissue sections were imaged on a Zeiss LSM700 confocal microscope using Fluar 10×/0.50NA, Plan-Apochromat 40×/1.4NA and 60 × /1.4NA oil-immersion objective lenses. Imaging was performed on 3–5 fields per tissue section. Optical sections and Z-projections were analyzed for every tissue section. Image acquisition was performed with Zen and final image composites and maximum intensity Z-projections were generated with Zen software and ImageJ. Imaris was used for 3D rendering.
Live cell imaging
FACS-purified GFP+ cells from the lin- stromal fraction of PdgfrαCreR26mTmG mammary tissue were co-cultured with sorted tdTomato+ epithelial cells from Cre-R26mTmG mammary glands on top of a thin layer of phenol red-free matrigel (BD Biosciences) in a Lab-Tek II 4 chambered cover glass system (Nunc) in DMEM:F12 medium containing 5% FBS (GIBCO), insulin (Life Technologies), EGF (STEMCELL Technologies), bFGF (STEMCELL Technologies), hydrocortisone (STEMCELL Technologies), Rock inhibitor (Reagents Direct) in 5% oxygen conditions. After 4 days of organoid growth, cultures were treated with vehicle control (4 mM HCl + 0.1% BSA) or 100 ng/ml PDGFCC (R&D systems) and imaged overnight with Zen software using 20 × /0.8 Plan-Apochromat objective lens of an inverted motorized Zeiss AxioObserver microscope equipped with a stage top heated CO2 incubator.
Cell migration assay
In a modified Boyden Chamber assay, PdgfrαCreR26mTmG GFP+ stromal cells (40,000 cells/well) suspended in DMEM:F12 medium were placed on 6.5 mm transwell inserts with a 8.0 μm pore size and underside coated with 30μl of phenol red-free matrigel (BD Biociences) in 24 well plates (Corning). DMEM: F12 medium with vehicle control (4 mM HCl + 0.1% BSA) or 100 ng/ml PDGFCC (R&D systems) was added to the bottom chambers and cells incubated at 37 C for 4 h. Non-migrated cells were removed from the insert with a cotton swab, and migrated cells in the matrigel layer were fixed with paraformaldehyde and washed with PBS. GFP+ migrated cells were counted after imaging inserts on a cell imaging dish (Eppendorf) using a Zeiss LSM700 confocal microscope with Fluar 10X/0.50NA objective lens. Four microscope fields were counted per well and treatments performed in triplicate.
Mammary epithelial cells were FACS-sorted from adult wild-type non-reporter female mice and transplanted into the fourth inguinal PdgfrαCreERTR26mTmG or AdiponectinCreERTR26mTmG inducible lineage tracing mammary fat pads (10,000 cells per fat pad) after surgical severing of the fourth and fifth mammary gland connection and clearing of the endogenous mammary epithelium of 21 day old recipient females. After 8 weeks, recipient mice were injected once with TAM to induce Cre-mediated recombination and GFP labeling in the fat pad, rested for 1 week and then stimulated with hormones for 14 days or left untreated. Untreated mice were analyzed at the estrus phase. Resulting outgrowths were analyzed by confocal immunofluorescence on stained frozen sections of dissected mammary fat pads.
qPCR and ddPCR
RNA was prepared from FACS-sorted primary mammary cell fractions using the PicoPure RNA Isolation Kit (Arcturus). During isolation, samples were also treated with RNase-free DNase (Qiagen) to remove any contaminating DNA. The quality and concentration of RNA was determined by analysis with a NanoDrop 2000 Spectrometer (260/280 ratio; Thermo Scientific). For RT-PCR studies, total RNA was reverse transcribed into first strand cDNA and amplified using the SMARTer PCR cDNA Synthesis Kit and Advantage2 PCR Kit (Clontech). Relative quantification Real-time PCR (ΔΔCt) was performed on 2 ng of amplified and purified cDNA using an ABI PRISM 7900HT Sequence Detection System (Applied Biosystems). TaqMan gene expression assay mix (Applied Biosystems) containing unlabeled PCR primers and FAM-labeled TaqMan MGB probes were used to detect expression of Pdgfrα (Assay ID: Mm00440701_m1), Pdgfa (Assay ID: Mm01205760_m1), Pdgfb (Assay ID: Mm00440677_m1), Pdgfc (Assay ID: Mm00480205_m1) and β-actin (ACTB, Assay ID: Mm01205647_g1). Data were analyzed using Sequence Detection System software (v2.3; Applied Biosystems). The threshold cycle (CT) values were used to calculate relative RNA expression levels. Transcript levels were normalized to endogenous β-actin transcripts and compared to vehicle control stromal expression set at 1. First strand cDNA for droplet digital PCR (ddPCR) was prepared using qScript cDNA supermix (QuantaBio). The Bio-Rad QX200 droplet generator was used to generate 20μl of droplets, using the Bio-Rad protocol, from a mix of 5 ng cDNA, 2× ddPCR supermix (Bio-Rad), forward and reverse primers (450 nM), probe (FAM or HEX, 200 nM) and deionised distilled water (to 25μl). Droplets were cycled in a Bio-Rad C1000 at 95 °C for 10 min; 50× (94 °C −30 s, 61 °C − 60 s); 98 °C for 10 min, then 4 °C until analysis on the QX200 droplet reader using the QuantaSoft v1.4.0 software provided by Bio-Rad. Primers and probes for ddPCR are shown in Supplementary Table 1. All oligos were from Eurofins Genomics and all probes were from Integrated DNA Technologies.
RNA was isolated from FACS-sorted eGFP+ and tdTomato+ subsets from stromal and luminal mammary populations of individual mice using the PicoPure RNA Isolation Kit (Arcturus). RNA concentrations and RNA quality were measured using a bioanalyzer (Agilent) (0.095–193 ng/μl; RIN 1–10). cDNA was generated from 2 ng of RNA with the SMARTer stranded total RNA-seq kit – pico input mammalian (Takara) using a modified fragmentation time (0–4 min) to accommodate lower quality RNA. cDNA fragments were indexed and amplified before being cleaned up (Beckman) and depleted of ribosomal RNA (Takara). Following depletion, cDNA libraries were amplified over 15 cycles of PCR. cDNA libraries were sequenced on a NextSeq 500 system (Illumina) in paired-end 75 mode.
Alignment of raw sequence reads to the Mus musculus GRCm38.p5 GENCODE reference genome and the generation of gene level abundance estimates were performed using the STAR aligner (v.2.5.2a)57. Multivariate linear regression analysis was accomplished using the R package limma (v.3.32.2)58 and genes with Benjamini-Hochberg corrected P values less than 0.01 were considered as differentially expressed. KEGG pathway analysis was performed using the R package gprofiler (v.0.6.1)59 and top 10% most significantly enriched pathways were selected for comparison. Plots were generated using the BPG R package (v.5.7.1). All analyses and visualization were run in the R statistical environment (v.3.4.0).
Sample sizes were chosen based on previous experience with comparable experiments utilizing animal models that generated measurable and reproducible responses10,11. In every instance, n represents a distinct biological replicate unless otherwise stated. Data for biological replicates were acquired on the same day or pooled from independent days. Where possible, experiments were repeated at least two independent times with successful replication. Data were analyzed using GraphPad prism software and reported as mean ± standard error of the mean (s.e.m). Comparison of data between multiple groups was performed using one-way analysis of variance (ANOVA) followed by Tukey’s post-hoc multiple comparison test, and analysis between two groups was made using Student’s t-test (two-tailed). Statistical significance is recognized at p<0.05.
Further information on research design is available in the Nature Research Reporting Summary linked to this article.
Data that support the findings of this study are available from the corresponding author upon reasonable request. RNA-sequencing data are available from GEO under accession number GSE123714. The source data underlying Figs. 1b, e, i, 2f, g, i, j, 3d, e, 4c, f, i, l, 5b, 7b-g, j and Supplementary Figs. 1b and 8a, b are provided as a Source Data file.
Joshi, P. A., Di Grappa, M. A. & Khokha, R. Active allies: hormones, stem cells and the niche in adult mammopoiesis. Trends Endocrinol. Metab. 23, 299–309 (2012).
Stingl, J. & Caldas, C. Molecular heterogeneity of breast carcinomas and the cancer stem cell hypothesis. Nat. Rev. Cancer 7, 791–799 (2007).
Stingl, J. et al. Purification and unique properties of mammary epithelial stem cells. Nature 439, 993–997 (2006).
Shackleton, M. et al. Generation of a functional mammary gland from a single stem cell. Nature 439, 84–88 (2006).
Van Keymeulen, A. et al. Distinct stem cells contribute to mammary gland development and maintenance. Nature 479, 189–193 (2011).
Rios, A. C., Fu, N. Y., Lindeman, G. J. & Visvader, J. E. In situ identification of bipotent stem cells in the mammary gland. Nature 506, 322–327 (2014).
Wang, D. et al. Identification of multipotent mammary stem cells by protein C receptor expression. Nature 517, 81–84 (2015).
Wang, C., Christin, J. R., Oktay, M. H. & Guo, W. Lineage-biased stem cells maintain estrogen-receptor-positive and -negative mouse mammary luminal lineages. Cell Rep. 18, 2825–2835 (2017).
van Amerongen, R., Bowman, A. N. & Nusse, R. Developmental stage and time dictate the fate of Wnt/beta-catenin-responsive stem cells in the mammary gland. Cell. Stem. Cell. 11, 387–400 (2012).
Joshi, P. A. et al. Progesterone induces adult mammary stem cell expansion. Nature 465, 803–807 (2010).
Joshi, P. A. et al. RANK signaling amplifies WNT-responsive mammary progenitors through R-SPONDIN1. Stem Cell Rep. 5, 31–44 (2015).
Casey, A. E. et al. Mammary molecular portraits reveal lineage-specific features and progenitor cell vulnerabilities. J. Cell. Biol. 217, 2951–2974 (2018).
Parmar, H. & Cunha, G. R. Epithelial-stromal interactions in the mouse and human mammary gland in vivo. Endocr. Relat. Cancer 11, 437–458 (2004).
Wiseman, B. S. & Werb, Z. Stromal effects on mammary gland development and breast cancer. Science 296, 1046–1049 (2002).
Houthuijzen, J. M. & Jonkers, J. Cancer-associated fibroblasts as key regulators of the breast cancer tumor microenvironment. Cancer Metastas-. Rev. 37, 577–597 (2018).
Barcellos-Hoff, M. H. & Ravani, S. A. Irradiated mammary gland stroma promotes the expression of tumorigenic potential by unirradiated epithelial cells. Cancer Res. 60, 1254–1260 (2000).
Maffini, M. V., Soto, A. M., Calabro, J. M., Ucci, A. A. & Sonnenschein, C. The stroma as a crucial target in rat mammary gland carcinogenesis. J. Cell. Sci. 117, 1495–1502 (2004).
Gyorki, D. E., Asselin-Labat, M. L., van Rooijen, N., Lindeman, G. J. & Visvader, J. E. Resident macrophages influence stem cell activity in the mammary gland. Breast Cancer Res. 11, R62 (2009).
Zhao, C. et al. Stromal Gli2 activity coordinates a niche signaling program for mammary epithelial stem cells. Science 356, eaal3485 (2017). pii.
Landskroner-Eiger, S., Park, J., Israel, D., Pollard, J. W. & Scherer, P. E. Morphogenesis of the developing mammary gland: stage-dependent impact of adipocytes. Dev. Biol. 344, 968–978 (2010).
Couldrey, C. et al. Adipose tissue: a vital in vivo role in mammary gland development but not differentiation. Dev. Dyn. 223, 459–468 (2002).
Hepler, C., Vishvanath, L. & Gupta, R. K. Sorting out adipocyte precursors and their role in physiology and disease. Genes Dev. 31, 127–140 (2017).
Rodeheffer, M. S., Birsoy, K. & Friedman, J. M. Identification of white adipocyte progenitor cells in vivo. Cell 135, 240–249 (2008).
Lee, Y. H., Petkova, A. P., Mottillo, E. P. & Granneman, J. G. In vivo identification of bipotential adipocyte progenitors recruited by beta3-adrenoceptor activation and high-fat feeding. Cell. Metab. 15, 480–491 (2012).
Berry, R. & Rodeheffer, M. S. Characterization of the adipocyte cellular lineage in vivo. Nat. Cell Biol. 15, 302–308 (2013).
Andrae, J., Gallini, R. & Betsholtz, C. Role of platelet-derived growth factors in physiology and medicine. Genes Dev. 22, 1276–1312 (2008).
Hoch, R. V. & Soriano, P. Roles of PDGF in animal development. Development 130, 4769–4784 (2003).
Festa, E. et al. Adipocyte lineage cells contribute to the skin stem cell niche to drive hair cycling. Cell 146, 761–771 (2011).
Macias, H. & Hinck, L. Mammary gland development. Wiley Interdiscip. Rev. Dev. Biol. 1, 533–557 (2012).
Shehata, M. et al. Phenotypic and functional characterization of the luminal cell hierarchy of the mammary gland. Breast Cancer Res. 14, R134 (2012).
Sleeman, K. E. et al. Dissociation of estrogen receptor expression and in vivo stem cell activity in the mammary gland. J. Cell. Biol. 176, 19–26 (2007).
Asselin-Labat, M. L. et al. Control of mammary stem cell function by steroid hormone signalling. Nature 465, 798–802 (2010).
Visvader, J. E. & Stingl, J. Mammary stem cells and the differentiation hierarchy: current status and perspectives. Genes Dev. 28, 1143–1158 (2014).
Hudak, C. S. et al. Pref-1 marks very early mesenchymal precursors required for adipose tissue development and expansion. Cell Rep. 8, 678–687 (2014).
Gulyaeva, O., Nguyen, H., Sambeat, A., Heydari, K. & Sul, H. S. Sox9-Meis1 inactivation is required for adipogenesis, advancing Pref-1(+) to PDGFRalpha(+) cells. Cell Rep. 25, 1002–1017 e1004 (2018).
Jeffery, E. et al. Characterization of Cre recombinase models for the study of adipose tissue. Adipocyte 3, 206–211 (2014).
Joshi, P. A., Chang, H. & Hamel, P. A. Loss of Alx4, a stromally-restricted homeodomain protein, impairs mammary epithelial morphogenesis. Dev. Biol. 297, 284–294 (2006).
De Pascalis, C. & Etienne-Manneville, S. Single and collective cell migration: the mechanics of adhesions. Mol. Biol. Cell 28, 1833–1846 (2017).
Maritzen, T., Schachtner, H. & Legler, D. F. On the move: endocytic trafficking in cell migration. Cell. Mol. Life Sci. 72, 2119–2134 (2015).
Bunney, T. D. & Katan, M. Phosphoinositide signalling in cancer: beyond PI3K and PTEN. Nat. Rev. Cancer 10, 342–352 (2010).
Fraser, J. K., Wulur, I., Alfonso, Z. & Hedrick, M. H. Fat tissue: an underappreciated source of stem cells for biotechnology. Trends Biotechnol. 24, 150–154 (2006).
Safford, K. M. et al. Neurogenic differentiation of murine and human adipose-derived stromal cells. Biochem. Biophys. Res. Commun. 294, 371–379 (2002).
Lue, J. et al. Transdifferentiation of adipose-derived stem cells into hepatocytes: a new approach. Liver Int. 30, 913–922 (2010).
Morroni, M. et al. Reversible transdifferentiation of secretory epithelial cells into adipocytes in the mammary gland. Proc. Natl Acad. Sci. USA 101, 16801–16806 (2004).
Ishay-Ronen, D. et al. Gain fat-lose metastasis: converting invasive breast cancer cells into adipocytes inhibits cancer metastasis. Cancer Cell. 35, 17–32 e16 (2019).
Vona-Davis, L., Howard-McNatt, M. & Rose, D. P. Adiposity, type 2 diabetes and the metabolic syndrome in breast cancer. Obes. Rev. 8, 395–408 (2007).
Renehan, A. G., Zwahlen, M. & Egger, M. Adiposity and cancer risk: new mechanistic insights from epidemiology. Nat. Rev. Cancer 15, 484–498 (2015).
Zeve, D., Tang, W. & Graff, J. Fighting fat with fat: the expanding field of adipose stem cells. Cell. Stem. Cell. 5, 472–481 (2009).
Park, J., Morley, T. S., Kim, M., Clegg, D. J. & Scherer, P. E. Obesity and cancer-mechanisms underlying tumour progression and recurrence. Nat. Rev. Endocrinol. 10, 455–465 (2014).
Bertolini, F., Orecchioni, S., Petit, J. Y. & Kolonin, M. G. Obesity, proinflammatory mediators, adipose tissue progenitors, and breast cancer. Curr. Opin. Oncol. 26, 545–550 (2014).
Morsing, M. et al. Evidence of two distinct functionally specialized fibroblast lineages in breast stroma. Breast Cancer Res. 18, 108 (2016).
Cardiff, R. D. & Wellings, S. R. The comparative pathology of human and mouse mammary glands. J. Mammary Gland Biol. Neoplasia 4, 105–122 (1999).
Nolan, E. et al. RANK ligand as a potential target for breast cancer prevention in BRCA1-mutation carriers. Nat. Med. 22, 933–939 (2016).
Sigl, V. et al. RANKL/RANK control Brca1 mutation-driven mammary tumors. Cell Res. 26, 761–774 (2016).
Kelsey, J. L., Gammon, M. D. & John, E. M. Reproductive factors and breast cancer. Epidemiol. Rev. 15, 36–47 (1993).
van Kruijsdijk, R. C., van der Wall, E. & Visseren, F. L. Obesity and cancer: the role of dysfunctional adipose tissue. Cancer Epidemiol. Biomark. Prev. 18, 2569–2578 (2009).
Dobin, A. et al. STAR: ultrafast universal RNA-seq aligner. Bioinformatics 29, (15–21 (2013).
Ritchie, M. E. et al. limma powers differential expression analyses for RNA-sequencing and microarray studies. Nucleic Acids Res. 43, e47 (2015).
Reimand, J. et al. g:Profiler-a web server for functional interpretation of gene lists (2016 update). Nucleic Acids Res. 44, W83–W89 (2016).
This work was supported by grants to R.K. from the Canadian Cancer Society Research Institute (CCSRI) and Hold’Em For Life (Toronto). P.A.J. held a postdoctoral fellowship from the Canadian Cancer Society (CBCF, CCSRI). K.K. holds a Canadian Institutes of Health Research (CIHR) postdoctoral fellowship. PCB was supported by CIHR and TFRI New Investigator Awards. O.G. and H.S.S. are supported by NIDDK. The authors thank Julie Livingstone at the OICR for assistance with RNA-seq analysis, Princess Margaret Genomics Centre in particular Nicholas Khuu for RNA sequencing, Aleks Spurmanis and Frances Tong of the Princess Margaret flow cytometry facility for cell sorting, and Jaselyn Becz of the UHN Animal Resource Centre for technical assistance.
The authors declare no competing interests.
Journal peer review information: Nature Communications thanks the anonymous reviewer(s) for their contribution to the peer review of this work. Peer reviewer reports are available.
Publisher’s note: Springer Nature remains neutral with regard to jurisdictional claims in published maps and institutional affiliations.
Rights and permissions
Open Access This article is licensed under a Creative Commons Attribution 4.0 International License, which permits use, sharing, adaptation, distribution and reproduction in any medium or format, as long as you give appropriate credit to the original author(s) and the source, provide a link to the Creative Commons license, and indicate if changes were made. The images or other third party material in this article are included in the article’s Creative Commons license, unless indicated otherwise in a credit line to the material. If material is not included in the article’s Creative Commons license and your intended use is not permitted by statutory regulation or exceeds the permitted use, you will need to obtain permission directly from the copyright holder. To view a copy of this license, visit http://creativecommons.org/licenses/by/4.0/.
About this article
Cite this article
Joshi, P.A., Waterhouse, P.D., Kasaian, K. et al. PDGFRα+ stromal adipocyte progenitors transition into epithelial cells during lobulo-alveologenesis in the murine mammary gland. Nat Commun 10, 1760 (2019). https://doi.org/10.1038/s41467-019-09748-z
This article is cited by
Mammalian tumor-like organs. 2. Mammalian adipose has many tumor features and obesity is a tumor-like process
Infectious Agents and Cancer (2022)
Identification of a rare Gli1+ progenitor cell population contributing to liver regeneration during chronic injury
Cell Discovery (2022)
Mammary epithelial cells have lineage-rooted metabolic identities
Nature Metabolism (2021)
Systemic alterations play a dominant role in epigenetic predisposition to breast cancer in offspring of obese fathers and is transmitted to a second generation
Scientific Reports (2021)
Mammary gland adipocytes in lactation cycle, obesity and breast cancer
Reviews in Endocrine and Metabolic Disorders (2021)
By submitting a comment you agree to abide by our Terms and Community Guidelines. If you find something abusive or that does not comply with our terms or guidelines please flag it as inappropriate.