Dual Mechanisms of LYN Kinase Dysregulation Drive Aggressive Behavior in Breast Cancer Cells

Summary The SRC-family kinase LYN is highly expressed in triple-negative/basal-like breast cancer (TNBC) and in the cell of origin of these tumors, c-KIT-positive luminal progenitors. Here, we demonstrate LYN is a downstream effector of c-KIT in normal mammary cells and protective of apoptosis upon genotoxic stress. LYN activity is modulated by PIN1, a prolyl isomerase, and in BRCA1 mutant TNBC PIN1 upregulation activates LYN independently of c-KIT. Furthermore, the full-length LYN splice isoform (as opposed to the Δaa25–45 variant) drives migration and invasion of aggressive TNBC cells, while the ratio of splice variants is informative for breast cancer-specific survival across all breast cancers. Thus, dual mechanisms—uncoupling from upstream signals and splice isoform ratios—drive the activity of LYN in aggressive breast cancers.


Correspondence
In Brief Tornillo et al. show that in aggressive breast cancers, LYN activity is deregulated by a change in patterns of splice isoform expression. In BRCA1dysfunctional breast cancers, LYN activity is upregulated by a prolyl isomerase (PIN1) that is normally repressed by BRCA1.

INTRODUCTION
Breast cancers molecularly classified as basal-like breast cancer typically display the triple (ER/PR/HER2)-negative (TNBC) phenotype (Badve et al., 2011). The molecular etiology of sporadic TNBC is still poorly understood, although germline BRCA1 mutations predispose to TNBC, and BRCA1 silencing or dysfunction in the BRCA1 pathway can be found in sporadic TNBC (Badve et al., 2011). Limited therapeutic options are available for TNBC; chemotherapy is often initially beneficial, but TNBC has a high risk of relapse (Liedtke et al., 2008), emphasizing the need to elucidate its biology and identify targets for novel treatment options.
The mammary epithelium consists of luminal cells, including ER-negative (ERÀ) progenitor-like and ER-positive (ER+) differentiated cells, and basal cells. TNBC likely originates from luminal ERÀ progenitors, and the gene expression profile of both BRCA1 mutation-associated and sporadic TNBC reflects a luminal progenitor-like profile (Lim et al., 2009;Molyneux et al., 2010). Elucidating the molecular regulation of this cell subset is important to understand not only the normal mammary cell homeostasis but also the origins of TNBC.
Mammary ERÀ luminal progenitors are characterized by expression of the membrane tyrosine kinase receptor c-KIT Smart et al., 2011), which is required for growth and survival of these cells Tornillo et al., 2013) as well as the SRC family tyrosine kinase (SFK) LYN (Bach et al., 2017;Regan et al., 2012;Smart et al., 2011), a known effector of c-KIT signaling in hematopoietic cells (Shivakrupa and Linnekin, 2005). Other SFKs are expressed in the mammary epithelium, but other than LYN, only FYN has an expression pattern restricted to a specific population (basal epithelial cells) (Bach et al., 2017;Kendrick et al., 2008). Based on this co-expression, a c-KIT-LYN signaling axis in mammary epithelial progenitors is proposed.
Previous studies have largely focused on LYN function in hematopoietic cells and leukemia, and persistent activation and/or deregulation of LYN has been associated with imatinib resistance in BCR-ABL+ leukemia (Wu et al., 2008). In breast cancer, LYN has been reported as overexpressed and a potential drug target in TNBC by several studies (Choi et al., 2010;Hochgrä fe et al., 2010;Molyneux et al., 2010;Regan et al., 2012;Smart et al., 2011). LYN point mutations in breast cancer are rare (0.6%) (https://cancer.sanger.ac.uk/cosmic), but have been associated with anti-estrogen resistance in a subset of ER+ tumors (Schwarz et al., 2014); only 6%-10% of breast cancers show LYN amplification (http://www.cbioportal.org/index. do; https://cancer.sanger.ac.uk/cosmic). Other mechanisms contributing to the underlying LYN dysregulation in TNBC remain to be defined, as does the potential wider role of LYN in breast cancer.
Here we demonstrate that LYN kinase is a transducer of c-KIT growth signals in the normal mammary epithelium. We show that LYN can also be activated by prolyl isomerase 1 (PIN1), normally transcriptionally repressed by BRCA1. In BRCA1-deficient TNBC, loss of this transcriptional repression results in increased PIN1 levels and thus in LYN activation independently of c-KIT. Furthermore, we address the role of the two LYN splice isoforms in breast cancer and find that only full-length LYN (LYNA), as opposed to LYN D25-45 (LYNB), promotes cell migration and invasion. LYNA is expressed more highly in TNBC than other breast cancer types; however, we find that a higher ratio of LYNA over LYNB is present in breast cancers of patients with shorter survival times, irrespective of tumor subtype. Therefore, our findings demonstrate dual mechanisms, uncoupling from upstream signals and changing splice isoform ratios, driving the activity of LYN in aggressive breast cancers. These mechanisms have the potential to be targeted therapeutically, and the LYNA::B ratio is a biomarker that could identify patients who would benefit from such interventions.

LYN Kinase Is Regulated by c-KIT and Promotes Growth of Normal Mammary Epithelial Cells
To define the major components of the c-KIT signaling network in the mammary epithelium, we examined expression of c-KIT and its ligand stem cell factor (SCF) in normal mouse mammary cell populations ( Figure 1A). The two splice variants of c-KIT, GNNK+,and GNNKÀ, were expressed primarily in luminal cells (particularly in the ERÀ luminal subpopulation) ( Figure 1B). The two SCF isoforms, soluble SCF (sSCF) and membrane-bound SCF (mSCF), were present at low levels in luminal cells, whereas basal cells showed the highest levels of total SCF, with almost exclusive expression of the sSCF form ( Figures 1B and 1C).
LYN is a key effector of c-KIT signaling in hematopoietic cells, and LYN expression and c-KIT expression in the mammary gland are correlated Roskoski, 2005). LYN exists in two isoforms, LYNA (full-length LYN) and LYNB (LYN D25-45 ) (Figure 1D). When expression of these isoforms was analyzed by semiquantitative RT-PCR, both LynA and LynB were found in all mammary epithelial populations; however, there was an association between higher LynA and c-Kit expression in the luminal ERÀ compartment ( Figure 1B). Therefore, the expression pattern of c-KIT, SCF, and full-length LYN in the mammary epithelium indicated the existence of a basal-to-luminal paracrine c-KIT signaling network, mediated by the soluble form of SCF (sSCF), along with an enrichment of a potential c-KIT effector, LYN, in the SCF-responsive luminal cells.
To determine the signaling cascade activated by c-KIT, we treated primary mouse mammary epithelial cells with SCF and assessed the phosphorylation status of a series of previously described c-KIT effectors (Roskoski, 2005). Addition of SCF caused a marked increase in c-KIT phosphorylation, as well as upregulation of phosphorylation levels of JAK2, STAT3, AKT, and ERK1/2 with distinctive kinetics ( Figure 1E). Phosphorylation levels of LYN at its positive regulatory site Y397 were elevated approximately 6-fold within 60 min of stimulation with SCF (Figure 1F), and SCF treatment induced an increase in LYN kinase activity as measured by an immunoprecipitation (IP) kinase assay ( Figure 1G). Conversely, c-KIT inhibition, by using short hairpin RNA (shRNA) against c-KIT or a specific anti-c-KIT blocking antibody (ACK2), led to a significant decrease in LYN phosphorylation ( Figures 1H and 1I; Figure S1A).
Because c-KIT is required for growth of normal mammary cells in vitro  and positively regulated LYN activity, we tested whether LYN depletion also affected mammary cell growth. Following Lyn knockdown with two distinct shRNAs (shLyn1 or shLyn2) (Figure 2A), primary mouse mammary epithelial cells exhibited defective growth ( Figure 2B) and a significant reduction in the expression of the proliferation marker Ki67 ( Figure 2C). This effect was observed both in unsorted primary mammary epithelial cells and in the purified luminal ERÀ progenitor population (Figures 2D and 2E;Figure S1B). Furthermore, knockdown of LYN in the human normal mammary epithelial cell line, MCF10A, with two distinct shRNAs caused a significant reduction in relative cell growth and in Ki67 expression compared to shScrambled (shScr) controls ( Figures 2F and 2G), without obviously affecting acinar architecture ( Figure S1C).
We next tested the ability of a constitutively active LYN (Y508F) mutant to rescue c-KIT knockdown. Whereas overexpression of wild-type LYNA (LYNA WT) had no effect on the viability of c-KIT knockdown cells, constitutively active LYN (LYNA CA) rescued the growth defect ( Figure S2A). In addition, when we examined the ability of LYN-depleted cells to activate c-KIT downstream effectors in response to SCF, we found that LYN knockdown specifically interfered with AKT phosphorylation upon c-KIT stimulation ( Figure S2B). Overall, these findings support the model that c-KIT activates LYN kinase to transduce (A) Flow cytometry of primary mammary cells stained with CD45, CD24, and Sca-1 antibodies. CD45 + leukocytes (purple) were gated out (top plot), and CD45 À cells (bottom plot) were gated to define basal (CD24 +/low Sca-1 À , red), luminal ERÀ (CD24 +/high Sca-1 À , green), and luminal ER+ (CD24 +/high Sca-1 + , blue) epithelial cell populations. (B) Expression pattern of c-Kit, Scf, and Lyn splicing transcripts in mouse mammary cell populations. Semiquantitative RT-PCR data are representative of two independent isolates (four mice for each). Amplicons of the expected size using primers spanning the alternative exon for each gene are indicated. Gapdh was used as a control. (C) qRT-PCR gene expression analysis of Scf in mouse mammary cell populations using probes for both total Scf (membrane bound and soluble) or soluble Scf (sSCF) only. Data are from two independent isolates (four mice for each), presented as relative expression levels with leukocytes as the comparators. (D) Schematic of LYN isoforms showing the 21-amino acid insertion (black residues) in the N-terminal domain of LYNA. (E) Representative western blot analysis and quantitation of c-KIT, JAK2, STAT3, AKT, and ERK1/2 phosphorylation levels in protein extracts from primary mouse mammary organoids cultured on Matrigel and stimulated with SCF for the indicated times. Tubulin was used as loading control. (F and G) Representative western blot analysis and quantitation of LYN autophosphorylation (Y397) (F) and immunoprecipitation (IP) LYN kinase assay of protein extracts (G) from primary mouse mammary organoids cultured on Matrigel and stimulated with SCF for 0, 15, 30, and 60 min. (H and I) Western blot of c-Kit expression and LYN autophosphorylation (Y397) in primary mouse mammary organoids after transduction with control (shScr) or c-Kit knockdown (shKit1 and shKit2) lentiviruses (H) or following treatment with c-KIT blocking (ACK2) or immunoglobulin G (IgG) isotype (IgG Ctr) antibodies (I). Unless otherwise stated, blots are representative of three independent experiments (mean and SD; two-tailed unpaired t tests) (in E and F, t tests are relative to time 0). *p < 0.05; **p < 0.01; ***p < 0.001. See also Figure S1. pro-growth and survival signals and activate the AKT pathway in mammary epithelial cells.

LYN Is Required for Growth of BRCA1-Deficient Mammary Tumor Cells
We have previously demonstrated that Brca1 mutation-associated breast cancers originate from luminal ERÀ progenitors (Molyneux et al., 2010) and that c-KIT and LYN are expressed in mouse Brca1 mammary tumors . To determine whether Brca1 mutant cell growth depends on the activation of the c-KIT signaling pathway, primary mouse Brca1 mutant mammary tumor cells transduced with lentiviruses expressing either one of two shRNAs against c-Kit (shKit1 and shKit2) or a control shRNA (shScr) were analyzed. Despite reduced c-Kit expression, no change in cell growth was observed in shKit cells compared to shScr cells ( Figure S2C). Furthermore, unlike normal cells, c-Kit-depleted tumor cells had phospho-LYN levels similar to those of control cells ( Figure S2D) and treatment of Brca1 tumor cells with the ACK2 c-KIT blocking antibody did not alter LYN phosphorylation status ( Figure S2E; contrast with Figure 1I). Likewise, c-KIT knockdown failed to affect phospho-LYN levels in three human c-KIT-positive breast cancer cell lines with low BRCA1 levels: HCC38 (BRCA1 silenced by methylation), HCC1806, and MDA-MB-157 (BRCA1 low due to downregulation by microRNA [miRNA]) (Garcia et al., 2011;Li et al., 2013) ( Figure S3A). However, c-KIT knockdown in a c-KIT-positive BRCA1-wild-type cell line, HCC1187, suppressed LYN phosphorylation ( Figure S3A). These results indicate that in Brca1/BRCA1 tumor cells, at least in vitro, c-KIT is dispensable for growth and does not regulate LYN activity.
Next, we evaluated the effects of LYN knockdown on Brca1 tumor cell growth. LYN knockdown markedly impaired growth of mouse Brca1 tumor-derived cells in monolayer culture (Figure 3A) and in three-dimensional (3D) culture conditions on Matrigel ( Figure 3B). Staining of 3D-cultured tumor cells for the proliferation marker Ki67 showed that the number of proliferating cells was reduced by approximately 30% in shLyn-transduced cultures compared with control ( Figure 3C). The kinase activity of LYN was required for its pro-survival functions, because expression of shRNA-resistant wild-type LYNA (LYNA*WT) was able to rescue the effect of shLyn transduction, but expression of a kinase-dead LYNA (T410K) mutant (LYNA*KD) was unable to do so ( Figure 3D). The broad spectrum kinase inhibitor Dasatinib, which was able to block LYN Y397 phosphorylation in mammary epithelial cells in a dose-dependent manner (Figure S3B), inhibited growth of three mouse BRCA1 tumor-derived cell lines (half-maximal inhibitory concencetration [IC 50 ] 0.1-1 mM) and the human BRCA1 mutant HCC1937 line (IC 50 0.1 mM) ( Figures S3C and S3D).
Use of two short hairpins targeting human LYN ( Figure 3E) demonstrated that LYN knockdown in human breast cancer cells also significantly impaired cell growth in the BRCA1-mutated HCC1937 human breast cancer cell line ( Figure 3F) and in cells from a BRCA1 mutant breast cancer patient-derived xenograft (PDX) ( Figure 3G). These effects, therefore, were consistent in both mouse and human cells.
Because LYN blockade effectively suppressed tumor cell growth in vitro, we next evaluated the effects of blocking LYN activity in vivo. Intraperitoneal (i.p.) injection of Dasatinib strongly reduced LYN phosphorylation in the normal mammary epithelium of wild-type mice ( Figure S3E), and daily treatment with Dasatinib significantly inhibited growth of BlgCre Brca1 fl/fl p53 +/À tumors ( Figures S3F and S3G). Immunohistochemical staining for phospho-histone H3 (phospho-H3) showed a lower number of mitotic cells in Dasatinib-treated compared to vehicle-treated tumors ( Figure S3H).
Reduction of cell numbers following constitutive Lyn knockdown made testing the effects of specific Lyn depletion by shRNA on tumor cell growth in vivo difficult. Therefore, a conditional Lyn knockdown system in which mouse Brca1 tumor cells expressed shRNA against Lyn under the control of doxycycline was established. Analysis of Lyn transcript levels after exposure to doxycycline confirmed that Lyn expression was reduced in inducible shLyn-carrying cells in the presence of doxycycline (C) Ki67 immunofluorescence staining (green) of control (shScr)-and shLyn-carrying mammary organoids 6 days after lentiviral transduction (DAPI nuclear counterstaining). Representative images and quantification of the percentage of Ki67-positive cells. Scale bar, 20 mm. (D) Colony-forming potential of unfractionated primary mammary epithelial cells (all epithelial) or basal, luminal ERÀ, and luminal ER+ subpopulations. 5,000 cells from each fraction were plated on Matrigel, and colony numbers were determined after 12-14 days. (E) Growth inhibition of unfractionated primary mammary epithelial cells (all epithelial) or the luminal ERÀ fraction transduced with control (shScr) or Lyn knockdown (shLyn1 and shLyn2) lentiviruses and seeded onto Matrigel. Cell growth was assessed after 12-14 days. Representative images, left (scale bar, 100 mm); quantitation, right. (F) Growth inhibition of MCF10A cells transduced with lentiviral vectors carrying control shRNA (shScr) or shRNA against LYN (shLyn1 and shLyn2). Transduced cells were grown in 3D on Matrigel, and relative cell numbers were assessed after 12 days of culture. Representative images of acinar structures (day 12) derived from shScr, shLyn1, or shLyn2 cells are shown (scale bar, 100 mm), together with CellTiterGlo quantitation and assessment of LYN knockdown by western blot (GAPDH loading control). (G) Confocal microscope analysis of Ki67 immunofluorescence-stained shScr, shLyn1, or shLyn2 knockdown MCF10A cells at day 4 of culture in 3D with quantitation. DAPI was used for counterstaining. Scale bar, 20 mm. Blots are representative of three independent experiments. Quantitation, mean and SD (n = 3; two-tailed unpaired t tests) except for gene expression analysis by quantitative real-time RT-PCR (mean ± 95% confidence intervals; significance of real-time RT-PCR data was determined from confidence intervals; n = 3 independent experiments for each of 3 technical replicates per sample) (Cumming et al., 2007). *p < 0.05; **p < 0.01; ***p < 0.001. See also Figures S1-S3.
( Figure 3H). Upon orthotopic cell injection in immunodeficient mice, administration of doxycycline resulted in a significant decrease in the growth of tumors derived from cells carrying inducible anti-Lyn shRNA ( Figure 3I). Staining of tumor sections for the mitotic cell marker phospho-H3 revealed a reduction in the number of mitotic cells in samples from doxycycline-treated shLyn tumors compared with controls ( Figure S3I). Therefore, LYN kinase depletion suppresses Brca1 mammary tumor cell growth both in vitro and in vivo.
Brca1 Depletion Leads to Upregulation of LYN Kinase Activity in a PIN1-Dependent Manner Our data show that in normal mammary epithelial cells, LYN kinase activity is under the strict control of the c-KIT receptor, whereas in Brca1 mutant tumor cells, LYN functions independently of c-KIT. We hypothesized that inactivation of Brca1 might contribute to dysregulation of LYN kinase activity. First, we analyzed a panel of TNBC cell lines for LYN and phospho-LYN (Y397) levels. Three of the lines (MDA-MB-436, SUM-149, and HCC1937) carry inactivating BRCA1 mutations, one (HCC38) has BRCA1 promoter methylation, four (MDA-MB-157, HCC1806, MDA-MB-468, and HCC70) have been reported as having low BRCA1 expression (Buckley et al., 2016;Garcia et al., 2011;Gong et al., 2015;Li et al., 2013), and six (MDA-MB-231, MDA-MB-453, BT-20, BT-549, HCC1143, and HCC1187) are BRCA1 wild-type. Total LYN levels were variable across the lines; however, when phospho-LYN levels were normalized to total LYN, TNBC cells with defective BRCA1 had significantly higher levels of phospho-LYN than those of wildtype cells ( Figure 4A). Furthermore, Brca1 knockdown in primary (normal) mouse mammary epithelial cells resulted in increased LYN phosphorylation but unchanged c-KIT phosphorylation ( Figure 4B). Conversely, forced overexpression of hemagglutinin-tagged BRCA1 (HA-BRCA1) in primary mammary epithelial cells suppressed LYN phosphorylation ( Figure 4C).
The prolyl isomerase PIN1 recognizes specific serine-proline or threonine-proline sequences in proteins, changing the conformation of the prolines within these sequences and resulting in altered activity of the target protein (Zhou and Lu, 2016). LYN contains potential PIN1 consensus target sequences (Pro197 and Pro229), and PIN1 is transcriptionally repressed by BRCA1 (MacLachlan et al., 2000). Therefore, we hypothesized that increased LYN activity following BRCA1 inactivation or depletion results from increased PIN1 levels and that PIN1 was activating LYN. To test this, we first used phospho-protein arrays to demonstrate that both BRCA1 overexpression and PIN1 knockdown in MDA-MB-468 cells resulted in a significant reduction in phosphorylation of LYN, but not its close family member SRC ( Figures S4A and S4B). Moreover, we confirmed that BRCA1 suppresses PIN1 expression by overexpressing BRCA1 in MDA-MB-468 cells and showing that PIN1 mRNA levels were reduced by approximately 50% ( Figure S4C). We also compared PIN1 levels in mouse Brca1 tumor cells and normal mouse mammary epithelium and confirmed that PIN1 levels were significantly higher in the tumor cells ( Figure S4D).
Next, we stained a tissue microarray consisting of 15 germline BRCA1 mutant and 15 sporadic TNBC cases. Cases from BRCA1 patients showed, overall, significantly more intense PIN1 staining than did sporadic tumors ( Figures 4D and 4E). Given our findings that BRCA1 loss results in PIN1 upregulation, we hypothesized that even in sporadic breast cancers not linked to germline BRCA1 mutation but that have low BRCA1 levels through other mechanisms, levels of BRCA1 and PIN1 expression would be inversely correlated. We therefore Figure 3. LYN Activity Is Required for Growth of Brca1 Tumor Cells (A) Primary cells isolated from three distinct BlgCre Brca1 fl/fl p53 +/À mouse mammary tumors (1-3) were transduced with control (shScr) or Lyn knockdown (shLyn1 and shLyn2) lentiviruses, seeded at low density in adherent conditions (2D), and stained with crystal violet after 6 days. Viable cell density was determined by absorbance measurement following solubilization of the dye. Representative images of tumor cell colonies at day 6 of culture are shown. (B) shScr-, shLyn1-, or shLyn2-transduced BlgCre Brca1 fl/fl p53 +/À tumor cells (1-3) seeded in Matrigel (3D) were assessed for growth after 6 days. Graphs show cell number assessed at day 5 of culture relative to shScr cells. (C) Ki67 immunofluorescence staining (green) of control (shScr)-and shLyn-transduced BlgCre Brca1 fl/fl p53 +/À tumor cells in 3D culture 6 days after lentiviral transduction. Representative images and quantification of the percentage of Ki67-positive cells (n = 3). Scale bar, 20 mm. (D) Primary BlgCre Brca1 fl/fl p53 +/À mouse mammary tumor cells were transduced with either lentiviral shScr and empty expression vectors (shScr), shLyn and empty expression vectors (shLyn), or shLyn and expression vectors carrying either an shLyn-resistant form (indicated by an asterisk) of wild-type LYNA (shLyn + LYNA*WT) or a kinase-dead LYNA mutant (shLyn + LYNA*KD). LYN protein levels determined by western blot 6 days after transduction. The graph shows cell number assessed at day 5 of culture relative to shScr cells. (E) HCC1937 cells were transduced with control (shScr) or Lyn knockdown (shLyn1 and shLyn2) lentiviruses and tested for LYN expression levels by western blot after 6 days. (F) shScr-, shLyn1-, or shLyn2-transduced HCC1937 cells were seeded at low density in adherent conditions. Viable cell density was determined after 7 days as in (A). Representative images show tumor cell colonies at day 7 of culture. (G) BRCA1 mutant PDX-derived cells (BCM 3887) were transduced with control (shScr) or LYN knockdown (shLyn1 and shLyn2) lentiviruses and tested for cell viability after 10-12 days of culture in 3D on Matrigel.
(H) Primary mouse BlgCre Brca1 fl/fl p53 +/À mammary tumor cells were transduced with pHIV-RFP-Tet repressor and pSEW-GFP-TO-H1 (carrying either shScr or shLyn) lentiviruses. Lyn levels were determined in cells transduced with either inducible shScr or shLyn and in either the presence or the absence of doxycycline (DOX) by qRT-PCR relative to shScr cells without DOX. (I) 250,000 inducible shScr-or shLyn-transduced cells were orthotopically injected into the fourth right mammary fat pad of nude mice. These were randomized to DOX treatment or normal diet, and tumor growth was monitored. Tumor volumes were calculated from caliper measurements of tumor width and length. Tumor growth curves (mean ± SEM) and representative images of endpoint tumors are shown. Blots are representative of three independent experiments. Unless otherwise stated, quantitation is shown as mean and SD (n = 3; for PDX cell experiments n = 3 cell isolations from 3 PDX implants in 3 mice; two-tailed unpaired t tests), except for gene expression analysis by quantitative real-time RT-PCR (mean ± 95% confidence intervals; significance of real-time RT-PCR data was determined from confidence intervals; n = 3 independent experiments for each of 3 technical replicates per sample) (Cumming et al., 2007). *p < 0.05; **p < 0.01; ***p < 0.001. See also Figure S3. investigated their expression patterns in sporadic TCGA breast cancer cases and, consistent with our hypothesis, observed an inverse correlation between BRCA1 and PIN1 expression levels ( Figure S4E).
To demonstrate a direct functional link between PIN1 expression and LYN activity, we knocked down PIN1 in primary mouse Brca1 null cells ( Figure 5A) and cells from a BRCA1 mutant human breast cancer cell line (HCC1937) ( Figure 5B) and the BRCA1 mutant PDX ( Figure 5C). In all cases, knockdown of PIN1 decreased active LYN phosphorylation and cell survival, mimicking the effect of LYN knockdown, but it did not change c-KIT phosphorylation.
Co-immunoprecipitation (coIP) demonstrated that in mouse Brca1 null tumor cells, PIN1 interacted with LYN ( Figure 5D). Furthermore, generation of mutants in putative PIN1 consensus target sequences ( Figure 5E) showed that proline-to-isoleucine mutation of either residue 197 or both 197 and 229 resulted in a significant increase in inhibitory LYN phosphorylation at the Y508 site ( Figure 5F).
We next assessed whether the PIN1-LYN regulatory mechanism is likely to be more widely applicable than just to BRCA1 breast cancer. We therefore knocked down PIN1 in BRCA2 null mammary epithelial cells and in a panel of BRCA1 and BRCA2 null ovarian cancer cells. PIN1 knockdown significantly reduced LYN Y397 phosphorylation in a human BRCA2 mutant breast cancer cell line ( Figure S5A) and in primary mouse Brca2 null tumor cells ( Figure S5B). However, knockdown of Brca2 in primary normal mouse mammary cells did not alter PIN1 or phospho-LYN levels ( Figure S5C). PIN1 knockdown suppressed LYN Y397 phosphorylation in COV 362 cells (BRCA1 mutant ovarian carcinoma) ( Figure S5D) and PEO-1 and PEO-4 cells (BRCA2 mutant ovarian carcinoma) (Figures S5E and S5F), but not in KURAMOCHI cells (BRCA2 mutant ovarian carcinoma) ( Figure S5G). Therefore, regulation of LYN by PIN1 is a general (but not universal) mechanism, but PIN1 is not regulated by BRCA2. These findings are consistent with transcriptional ac-tivity of BRCA1 being involved in PIN1 regulation, as previously shown (MacLachlan et al., 2000).
To further investigate the involvement of specific BRCA1 functional domains in the regulation of the PIN1-LYN axis, and the possibility that different clinically relevant BRCA1 mutants may have different effects on this axis, we re-expressed either the wild-type BRCA1 or clinically relevant BRCA1 missense mutants (C61G in the RING domain, L1407P in the CC motif, and A1708E in the BRCT domain) (Anantha et al., 2017) in the HCC1937 human BRCA1-deficient breast cancer cell line. We found that re-expression of both wild-type and C61G mutant BRCA1 resulted in both decreased PIN1 levels and decreased LYN phosphorylation, while expression of the L1407P and A1708E mutations showed no significant differences compared to control BRCA1 mutant cells ( Figure 5G). Therefore, mutation of the N-terminal RING domain (which disrupts binding to BARD1) does not alter the ability of BRCA1 to suppress the PIN1-LYN activation pathway. In contrast, mutation of the coiled-coil domain, affecting PALB2 binding (suggested to be critical for the activation of the BRCA1 transcriptional program, as well as for DNA repair) (Anantha et al., 2017;Gardini et al., 2014), and of the C-terminal BRCT domains, important for interactions with Abraxas, BRIP1, and CtIP (Anantha et al., 2017) and known to be important for BRCA1 transcriptional activity (Hayes et al., 2000;Iofrida et al., 2012), result in elevated levels of PIN1 and LYN activation. These support a model in which the transcriptional activity of BRCA1 is critical in the control of PIN1-LYN pathway activation.
Having established the BRCA1-PIN1-LYN axis, and given the important role of BRCA1 in repair of double-stranded DNA breaks, we examined whether LYN activity could affect the normal mammary cell response to DNA damage. Primary normal mouse mammary epithelial cells expressing LYNA CA were treated with the DNA damaging agent methyl methane sulfonate (MMS), which causes double-stranded breaks. Expression of LYNA CA led to a marked transient increase in Akt phosphorylation, suggesting elevated levels of survival signaling, and a significant reduction in cleaved PARP levels ( Figure S6A) and TUNEL staining ( Figure S6B), both markers of apoptosis, after MMS treatment relative to control cells. Consistent with this, levels of cleaved caspase-3 were significantly reduced in normal mammary cells expressing LYNA CA, compared to control cells, following treatment with 10 mM cisplatin ( Figure S6C) or exposure to 10 Gy of ionizing radiation ( Figure S6D). Blots in (B) and (C) are representative of three independent experiments. Quantitation is shown as mean and SD (n = 3; two-tailed unpaired t tests) except for gene expression analysis by quantitative real-time RT-PCR (mean ± 95% confidence intervals; significance of real-time RT-PCR data was determined from confidence intervals; n = 3 independent experiments for each of 3 technical replicates per sample) (Cumming et al., 2007). *p < 0.05; **p < 0.01. See also Figure S4.

LYNA Drives Breast Tumor Cell Aggressiveness
We next asked whether the two LYN isoforms, LYNA and LYNB (shown in detail in Figure S7A), play different roles in breast cancer biology, independent of the BRCA1-PIN1-LYN axis. First, we transiently expressed GFP-tagged variants of LYNA and LYNB in MDA-MB-231 cells. After 48 hr, cells were fixed, counterstained with DAPI, and analyzed by confocal microscopy. Both LYNA and LYNB were predominantly membrane localized, with additional foci of intracellular staining, under these conditions ( Figure S7B).
Next, we used a LYNA-specific shRNA to knock down LYNA expression in MDA-MB-231 cells. shLynA cells displayed an approximately 60% reduction in LYNA protein levels compared to control (shScr) cells ( Figure 6A). LYNA knockdown resulted in an overall decrease in cell proliferation ( Figure 6A) and a strong reduction in cell migration and invasion in vitro ( Figure 6B). To exclude the possibility that the impaired growth, migration, and invasion of shLynA knockdown cells was due to a reduction in total LYN levels, rather than depletion of the LYNA form, and to determine the specific contribution of each LYN variant to the malignant behavior of the cells, we used a knockdown and reconstitution approach. Total LYN was knocked down in MDA-MB-231 cells, and then either a LYNA or a LYNB variant (LYNA* or LYNB*) not targetable by shLyn was re-expressed. We assessed cell growth and the ability of the cells to migrate and invade relative to control cells. Total LYN knockdown led to a decrease in cell growth, but this could be rescued by either LYNA* or LYNB* ( Figure 6C), indicating that these two distinct LYN isoforms can compensate for each other in promoting tumor cell growth. LYN knockdown significantly reduced the ability of the cells to migrate and invade; this could be rescued by LYNA*; however, LYNB* was unable to do so ( Figure 6D). Therefore, while both LYN isoforms promoted tumor cell growth, only LYNA drove aggressive behavior in these cells.
To determine whether LYNA and LYNB may associate with different protein partners, and whether this might explain their different effects on migration and invasion, we carried out a mass spectrometry analysis of proteins that interact with the two isoforms. LYN was knocked down in MDA-MB-231 cells, and then either LYNA* or LYNB* was re-expressed. We also expressed a LYNA* variant, LYNA* Y32F ( Figure S7C). Y32 is located within the 21-amino acid segment present in LYNA and has been reported as being regulated by epidermal growth factor (EGF) signaling (Huang et al., 2013); if phosphorylation of this tyrosine was required for the differential behavior of LYNA compared to LYNB, then we would predict LYNA* Y32F would behave like LYNB. Cultures were established in duplicate, and one set was treated with EGF before lysis (Huang et al., 2013). LYN was immunoprecipitated from these eight conditions (LYN KD, LYNA*, LYNB*, and LYNA* Y32F ; all ±EGF), and lysates were analyzed by tandem mass tagging. The full results and differentially enriched proteins are provided in Table S1. There was little difference between the proteins that co-immunoprecipitated with LYNA* and LYNA* Y32F , arguing against the hypothesis that LYNA* Y32F was like LYNB ( Figure S7D). The outcome of the analysis of the LYNA*ÀEGF, LYNA*+EGF, LYNA* Y32F ÀEGF, and LYNA* Y32F +EGF pull-downs, four independent cell preparations, was similar. Furthermore, the list of co-immunoprecipitated proteins included eight previously characterized LYN-interacting proteins (ANKRD54, LIMA1, HNRNPK, MYH9, STAT3, PRKDC, EGFR, and HSP90AB1) (Hein et al., 2015;Hornbeck et al., 2015;Huang et al., 2005;Kumar et al., 1998;Mertins et al., 2016;Petschnigg et al., 2014;Taipale et al., 2012;Tauzin et al., 2008;Van Seuningen et al., 1995).
By comparing LYN knockdown samples with LYNA*-and LYNB*-expressing samples, several proteins were identified that were differentially enriched in LYNA* samples. Using a cutoff for analysis of proteins that were enriched >1.2-fold both in the LYNA* pull-down compared to the LYN KD pull-down and in the LYNA* pull-down compared to the LYNB* pull-down, we identified 20 candidate LYNA-interacting proteins. We carried out a gene ontology analysis using DAVID (Huang et al., 2009) of the differentially interacting proteins to begin to understand their functional significance. The list of proteins and the results of this analysis are provided in Table S1. Six proteins (ACTC1, ACTG2, KRT5, LIMA1, MYH3, and TUBA1A) are associated with the cytoskeleton and its regulation, and two proteins (LPXN and TNS1) are associated with integrins and cell adhesion. These findings suggest that LYNA and LYNB may interact differently with cell adhesions and the cytoskeleton, potentially explaining the effects of LYNA on migration and invasion. Representative western blots and quantitation of phospho-LYN (Y397) levels are shown. GAPDH was used as loading control. shScr-, shPin1#1-, and shPin1#2-transduced BlgCre Brca1 fl/fl p53 +/À tumor cells and HCC1937 cells were also seeded at low density in adherent conditions and stained with crystal violet after 6 days. Cell number was determined by absorbance measurement following solubilization of the dye. PDX-derived transduced cells were cultured for 10-12 days in 3D on Matrigel and then assayed for cell viability. (D) Protein extracts from primary BlgCre Brca1 fl/fl p53 +/À mouse tumor cells transduced with vectors carrying wild-type LYNA were subjected to immunoprecipitation by anti-PIN1 or control (IgG) antibodies. Total extracts (input) and immunoprecipitates (IPs) were probed for PIN1 and LYN by western blot. (E) Schematic of LYN showing the position of PIN1 consensus recognition sequences and the proline > isoleucine mutants generated. (F) Representative western blot analysis of LYN phosphorylation levels at the negative regulatory phosphorylation site (Y508) in primary BlgCre Brca1 fl/fl p53 +/À transduced with vectors carrying wild-type LYNA or LYNA proline mutants (LYN P229I, LYN P197I, or LYN P197I P229I). (G) Western blot analysis of LYN autophosphorylation and PIN1 levels in human HCC1937 cells transduced with either control (Ctr) lentivirus or virus-carrying HAtagged wild-type or mutant BRCA1 (C61G, A1708E, or L1407P). Blots are representative of three independent experiments. Quantitation is shown as mean and SD (n = 3; two-tailed unpaired t tests). *p < 0.05; **p < 0.01; ***p < 0.001. See also Figures S5 and S6.

LYN Splicing Is Regulated by ESRP1
To determine what might regulate the balance between LYNA and LYNB expression, we first examined Affymetrix Human Exon 1.0ST array gene expression profiles of a breast cancer cohort from Guy's Hospital, London, and the TNBC subset of these cancers. Cohorts were split into high-LYNA-and low-LYNA-expressing tumors (i.e., above and below median expression of Affymetrix probe 3098998, uniquely targeting the N-terminal region of LYNA), and the expression levels of 270 splicing regulators (the spliceosome) (Table S2) (Papasaikas et al., 2015) were interrogated. We found that in 'all breast cancers' ( Figure S8A) and the TNBC subset ( Figure S8B), high-LYNA tumors had significantly lower spliceosome levels than those of low-LYNA tumors, indicating that splicing in general might be compromised. Next, we examined the expression of a splicing regulatory protein (ESRP1/RBM35A) with putative consensus sequences in LYN intron 2 ( Figure S8C). We found that ESRP1 levels were lower in high-LYNA breast cancers as a whole (Figure S8D) and in the high-LYNA TNBC subset ( Figure S8E). When ESRP1 was knocked down in MCF7 cells ( Figure S8F), which normally have a LYNA::B ratio of <2, the A::B ratio was significantly increased to a mean of 2.5:1 ( Figure 6E). Furthermore, when ESRP1 was overexpressed in MDA-MB-231 cells, which normally have a LYNA::B ratio of >3, this ratio was significantly reduced ( Figure 6F). Therefore, a decrease in the expression of the spliceosome in TNBC, and in particular ESRP1, could result in an increased LYNA::B ratio.
Patients with a High Tumor LYNA::B Ratio Have Shorter Survival Because LYNA drives aggressive migratory and invasive properties in breast cancer, we asked whether total LYNA expression levels, the relative amounts of LYNA and LYNB, or the LYNA::B ratio might have prognostic potential.
First, we analyzed the relative expression of the LYNA and LYNB isoforms in samples of human normal mammary tissue, as well as triple-negative (TN) and ER+/PR+ primary breast cancer. The ratio of LYNA to LYNB transcripts was close to 1 in the normal samples, but LYNA was preferentially expressed in TNBC ( Figure S9A). No significant difference in relative LYNA:: LYNB expression was observed in ER+/PR+ tumors compared to normal samples ( Figure S9A). Similar results were observed in a small panel of human breast cancer cell lines (basal ERÀ MDA-MB-231, MDA-MB-468, and HCC1143 and luminal ER+ MCF7) ( Figure S9B). However, while we could be confident that the tumor samples and cell lines in this analysis were predominantly composed of tumor cells, the normal tissue samples had not been purified and likely contained a mixture of normal epithelial cell populations and non-epithelial cells. Therefore, for a more accurate assessment of the LYNA::B ratio in normal human tissue, we used established flow cytometry protocols to purify the basal, luminal progenitor, luminal ER+ differentiated, and stromal cell populations from reduction mammoplasty samples from four individuals (Figures 7A-7C; Figure S10). Analysis of LYNA::B demonstrated that the luminal progenitor population had a significantly higher ratio compared with the other populations and that the LYNA::B ratio in normal cells was in a similar range to that of the tumor samples.
To expand our analysis, we investigated a panel of breast cancer cell lines  and the Guy's Hospital TNBCenriched breast cancer cohort  for the expression of the LYNA isoform using the Affymetrix probe 3098998. The LYNA sequence was significantly more highly expressed in basal and claudin-low cell lines than in luminal cell lines ( Figure S9C), and in the Guy's dataset, it was more highly expressed in tumors classified by PAM50 (Parker et al., 2009) as basal ( Figure S9D) or by immunohistochemistry as TNBC ( Figure S9E).
When we investigated the distributions of LYNA::B ratios across all tumors, we noted that while most sample ratios were in the range seen in the purified normal breast cells ( Figure 7C), Blots are representative of three independent experiments. Quantitation is shown as mean and SD (n = 3; two-tailed unpaired t tests), except for gene expression analysis by quantitative real-time RT-PCR (mean ± 95% confidence intervals; significance of real-time RT-PCR data was determined from confidence intervals; n = 3 independent experiments for each of 3 technical replicates per sample) (Cumming et al., 2007). *p < 0.05; **p < 0.01; ***p < 0.001. See also Figures S7 and S8. there was a distinct population of breast cancers with a log2 RSEM expression ratio of >7 ( Figure 7F). When this population was compared for time to breast cancer-specific death with the remaining TCGA breast cancer cases, it had a shorter median time for survival (p = 0.032 for >7.3) ( Figure 7G).

DISCUSSION
Although it has been previously reported that LYN is one of the most highly expressed SFKs in the normal mammary gland (Bach et al., 2017;Kendrick et al., 2008;Smart et al., 2011), its function in this tissue has not previously been investigated. LYN associates with c-KIT in hematopoietic cells and participates in numerous SCF-induced responses by promoting either positive or negative downstream signaling, depending on cell type and context (Shivakrupa and Linnekin, 2005). Our results demonstrate that LYN is activated by c-KIT and is critical for SCF:c-KIT-dependent phosphorylation of AKT in mammary progenitors. However, given that LYN has been implicated in other signaling pathways promoting cell survival and proliferation (Shivakrupa and Linnekin, 2005), it cannot be ruled out that additional pathways in mammary progenitors may be regulated by LYN.
c-KIT+/ERÀ mammary luminal progenitors are considered the cell of origin of BRCA1-mutated and sporadic TNBC (Lim et al., 2009;Molyneux et al., 2010). Although c-Kit is highly expressed in Brca1 mutant mammary tumors Smart et al., 2011), as well as in a subset of breast cancers within the TNBC group (Jansson et al., 2014), targeting this receptor has not been an effective therapeutic approach (Yardley et al., 2009). Our findings may at least partly explain why these trials have failed. Although carriers of BRCA1 germline mutations have an 80% lifetime risk of breast cancer, such cases make a small contribution to breast cancer in the general population. However, BRCA1 was found to be silenced through promoter methylation in 14% of sporadic basal-like and 11% of nonbasal-like breast cancers, while in two special subtypes of TNBC, medullary and metaplastic breast cancer, promoter methylation was found in >60% of cases (Badve et al., 2011;Turner et al., 2007). Furthermore, BRCA1 mRNA expression was two-fold lower in TNBC compared to matched controls, and this was suggested to depend on upregulation of ID4, a negative regulator of BRCA1 transcription (Turner et al., 2007). BRCA1 levels can also be suppressed by other epigenetic mechanisms, such as activity of miRNAs (Garcia et al., 2011;Li et al., 2013). Therefore, activation of the PIN1-LYN axis by BRCA1 downregulation is more widely applicable than to BRCA1 germline mutation carriers alone.
PIN1 can be aberrantly activated in human cancers by various mechanisms, including changes in transcription, translation, and/or post-translational modifications (Zhou and Lu, 2016). In addition to being a target for BRCA1 transcriptional activity, PIN1 is a direct transcriptional target of E2F (Ryo et al., 2002). PIN1 mRNA stability is also inhibited by miRNAs, while the phosphorylation and/or sumoylation status of specific PIN1 residues has been reported to be critical for PIN1 substrate binding and/or catalytic activity (Zhou and Lu, 2016).
PIN1 specifically catalyzes cis-trans proline isomerization within phosphorylated Ser/Thr-Pro motifs with important effects on phosphorylation-dependent signaling. Numerous oncogenes and tumor suppressors are directly regulated by PIN1 (Zhou and Lu, 2016), and here we show that PIN1 is an important contributor to LYN hyperactivation in BRCA1 mutant tumor cells. Consistent with PIN1 substrates typically containing one or few target motifs, LYN has only two putative PIN1 consensus sites  and Ser 228 -Pro 229 ). LYN phosphorylation at Ser 196 is only predicted, but phosphorylation at Ser 228 has been previously observed during cell-cycle progression (Daub et al., 2008), although the specific kinase or kinases involved are still unknown. These two sites are located in the SH2 domain and in the SH2-Kinase domain linker segment, respectively, which are involved in intra-and/or intermolecular interactions critical for the regulation of the open-closed LYN conformation, suggesting that local structural changes upon proline isomerization are likely to affect LYN activation status. Our findings suggest that regulation of LYN by PIN1 is a widely applicable mechanism of regulation of this SFK but that SRC is not a target of PIN1 ( Figure S4B); whether other SFKs are PIN1 targets remains to be investigated.
The link between BRCA1 loss of function and LYN activation and the activation by LYN of signaling pathways that promote cell survival, growth, and invasion are important findings. In normal cells, the absence of functional BRCA1 results in genomic instability, which leads to p53 activation, followed by cell-cycle arrest and apoptosis (Roy et al., 2011), implying that additional molecular alterations are required for BRCA1 mutant  (Iriondo et al., 2015). Plot is representative of outcomes of four independent sorts. (B) Quantitation of ESR1 expression levels, confirming ESR1 is most highly expressed in the mature luminal population (mean + SD relative to mature luminal cells; n = 3 independent cell preparations; unpaired two-tailed t test; **p < 0.01). (C) Quantitation of the relative LYNA::B ratio (n = 4 independent cell preparations; paired two-tailed t test; *p < 0.05) in breast cell populations. cells to survive and undergo malignant transformation. Not surprisingly, TP53 mutations are frequently present in BRCA1associated mammary tumors (Roy et al., 2011). As LYN hyperactivation suppressed cell death induced by DNA damage, aberrant LYN activation following BRCA1 loss could facilitate neoplastic progression, allowing BRCA1 loss-of-function cells to survive long enough to accumulate TP53 genetic alterations. Furthermore, activation of AKT downstream of LYN has been linked to ubiquitination and degradation of the p53 protein (Dos Santos et al., 2013;Iqbal et al., 2010), and this would enable functional suppression of the p53 pathway in BRCA1 mutant cells before genetic pathway suppression. There is some evidence that LYN is generally anti-apoptotic (Aira et al., 2018), and this warrants further investigation in breast cancer.
Alternative splicing is a critical post-transcriptional regulatory mechanism for many cancer-associated genes (Bonomi et al., 2013). LYN kinase exists as two isoforms, full-length LYN (LYNA) and LYN D25-45 (LYNB), differing by a 21-amino acid insert found in the unique NH2-terminal domain (Alvarez-Errico et al., 2010). We have found that in breast epithelial cells, the balance between these transcripts is modulated by the splicing factor ESRP1. LYN has not been found among the ESRP1-regulated alternative spliced genes resulting from previous analyses (Shapiro et al., 2011;Warzecha et al., 2009Warzecha et al., , 2010, most likely due to the lack of representative probe sets in the array platforms used in those studies. Nevertheless, like LYN, known ESRP1 target genes play a role in cell motility, cell adhesion, and/or epithelial-mesenchymal transition (Shapiro et al., 2011;Warzecha et al., 2009Warzecha et al., , 2010, indicating that co-regulation by ESRP1 of splicing of transcripts for proteins that may function, together with LYN, in a pro-migratory and invasive pathway in TNBC cells. We find that patients with breast cancer with a high LYNA:: LYNB ratio have a shorter time to breast cancer death. Biologically, this clinical phenotype could be a result of LYNA conferring migratory and invasive properties on breast cancer cells. How alteration of the LYNA::LYNB ratio can generate signal outputs leading to cancer cell aggressiveness remains to be fully defined. Previous analysis of LYNA and LYNB function in mast cells revealed the two isoforms associate differentially with phosphoproteins (Alvarez-Errico et al., 2010), indicating that the 21-amino acid sequence governs protein interactions. Moreover, LYNA was more potent than LYNB in activating Phospholipase C gamma (PLCg) and downstream Ca 2+ signaling (Alvarez-Errico et al., 2010). In addition, unlike LYNB, LYNA kinase activity can be enhanced through phosphorylation by EGFR at a specific tyrosine residue (Y32) within the 21-amino acid insert (Huang et al., 2013). However, in an analysis of proteins differentially interacting with the LYN isoforms, we saw little effect of either EGF stimulation or Y32F mutation in the 21-amino acid insert. We did find that LYNA interacted more strongly with proteins associated with the cytoskeleton, integrins, and cell adhesion, pointing to differential effects of LYNA and LYNB on migration and invasion. This warrants further work. Identification of patients who will respond to targeted, novel, or repurposed therapies remains a major goal of clinical research. Our findings demonstrate that patients with BRCA1 dysfunction or with a high LYNA::B isoform ratio would be particularly likely to benefit from specific therapies targeting LYN ki-nase. Furthermore, our findings on the key dual mechanisms of LYN regulation, combined with knowledge of LYN interaction partners, will enable rational design of new compounds to specifically block the oncogenic signaling driven by LYN without the need to directly target the kinase domain, increasing treatment specificity and reducing the likelihood of off-target effects.

CONTACT FOR REAGENT AND RESOURCE SHARING
Further information and requests for resources and reagents should be directed to and will be fulfilled by the Lead Contact, Professor Matt Smalley (SmalleyMJ@cardiff.ac.uk).

Animals
All animal work was carried out under UK Home Office project and personal licenses following local ethical approval and in accordance with local and national guidelines, including ARRIVE guidelines. Normal primary mammary cells were prepared from fourth mammary fat pads of 10 week-old virgin female FVB mice. The BlgCre Brca1 fl/fl p53 +/À and BlgCre Brca2 fl/fl p53 fl/fl mice and the tumors they generate have been fully described previously (Hay et al., 2009;Molyneux et al., 2010).  Zhang et al., 2013) was passaged in NOD scid gamma (NGS) mice.
The BRCA1 breast tumor (n = 15) and normal triple negative breast cancer (n = 15) tissue microarray was prepared by the Northern Ireland Biobank under ethical approval number NIB17-0232.
RNA samples from human tumor tissue were obtained from Breast Cancer Now Tissue Bank. Normal tissue samples were from reduction mammoplasties, selected to contain > 50% epithelium. All tumor samples (10 ER+PR+HER2-and 10 Triple Negative) were from primary tumors of no specific type, grade III, from pre-menopausal patients.

Cell lines
Cells were maintained at 37 C in a 5% CO 2 atmosphere with the exception of MDA-MB-157, which were kept in L-15 medium with 10% FBS, streptomycin (100 ug/ml) and penicillin (100 U/ml) in a free gas exchange with atmospheric air.

METHOD DETAILS
Isolation of and culture of normal mouse mammary epithelial cells All animal work was carried out under UK Home Office project and personal licenses following local ethical approval and in accordance with local and national guidelines, including ARRIVE guidelines.
Single cells were prepared from fourth mammary fat pads of humanely killed 10 week-old virgin female FVB mice. Intramammary lymph nodes were removed prior to tissue collection. Fat pads were finely minced on a McIlwain Tissue Chopper and then digested for 1 hr at 37 C in 3 mg/ml collagenase A / 1.5 mg/ml trypsin (both from Sigma, Poole Dorset, UK) in serum-free L15 medium (ThermoFisher Scientific, Life Technologies, Paisley, UK) with gentle rotation. Tissue fragments ('organoids') released from the fat pad were washed and then incubated for 5 min in Red Blood Cell Lysis buffer (Sigma), washed and then plated for 1 hr at 37 C in DMEM/10%FBS (ThermoFisher) to partially purify fibroblasts by differential attachment. Organoids were then poured off, pelleted, washed twice with versene (ThermoFisher) and then incubated for 15 min in serum-free Joklik's Low Calcium medium (Sigma) at 37 C. They were then pelleted and resuspended in 2mls of 0.25% trypsin / 0.02% EDTA in HBSS (Sigma) and incubated for two min 37 C to release single epithelial cells. 5 ml of 5 mg/ml DNase I (Sigma) in serum-free L15 was then added to digest DNA liberated from any lysed cells. Single epithelial cells were then pelleted and washed in L15/10% FBS (ThermoFisher Scientific, Life Technologies, Paisley, UK) and then resuspended at 10 6 cells/ml in L15/10% FBS Smalley, 2010;Smalley et al., 2012).
Phase-contrast images were taken using a Leica MI6000B microscope (10X PH1 objective) and the LAS AF software.
Preparation and flow cytometric separation of normal breast cells from reduction mammoplasty Normal breast tissue was obtained from pre-menopausal women undergoing reduction mammoplasty, with no previous history of breast cancer, who gave their informed consent. All samples were confirmed by histopathological examination to be free of malignancy. Immediately upon arrival at the laboratory, breast tissue was cut up manually into small pieces (approximately 0.5 cm cubed). Breast material was incubated in an equal volume of Dulbecco's modified Eagle's medium (DMEM) (GIBCO) supplemented with 5% fetal calf serum (FCS) and collagenase (Type I, Sigma) to a final concentration of 0.2 mg/ml, and digested (while shaking) overnight at 37 C. Following enzyme digestion, breast cells were washed and the organoids separated from any undigested material. The organoids were then isolated from blood cells, fibroblasts, and endothelial cells by sequential filtration and back flushing from 140 and 53 mm pore size polyester monofilament meshes. Organoids were then disaggregated with 0.05% trypsin-EDTA and finally filtered through a 40 mm sieve (BD) to yield a predominantly single cell suspension. Cells were immediately processed for flow cytometric cell sorting on the basis of CD49f, ESA and 7-AAD staining (see Figure 7 and Figure S10) (Iriondo et al., 2015). For CD49f/ESA staining, FITC-conjugated anti-ESA antibody and APC-conjugated anti-CD49f antibody were used (see Key Resources Table). In all cases, control samples were stained with isotype-matched control antibodies; the viability dye 7-aminoactinomycin D (7AAD) (BD) was used for dead cell exclusion and fluorescence minus one (FMO) controls were used to define the gates (Iriondo et al., 2015). In all cases, cells were analyzed and sorted using a FACSAria (Becton Dickinson) flow cytometer. Data were analyzed using FACSDiva software.

Primary tumor cell isolation and culture
Primary epithelial cells (from three distinct tumors (namely #1, #2, #3) from each mouse model or from three PDX implants) were obtained using the gentle MACS TM Dissociator and Mouse Tumor dissociation kit (Miltenyi Biotec, Bisley, Surrey, UK) following the manufacturer's recommendations using the protocol for 'Dissociation of Tough Tumors' for mouse tumors and the protocol for 'Dissociation of Soft and Medium Tumors' for the PDX. To ensure efficient dissociation volumes of Enzyme D, Enzyme R and Enzyme A were scaled up according to the size of the tumor piece (100 mL, 50 mL and 12.5 mL respectively per each 0.5 cm 3 ). The optional steps -the short spin for collection of the dissociated material at the bottom of the MACS tube and red blood cell lysis -were included in the procedure.
Mouse cells were cultured in complete growth medium in 2D adherent conditions for expansion or in 3D for functional studies. Cells up to passage 5 were used for all the experiments in this study. Freshly isolated human PDX cells were grown in HuMEC Ready Medium (Thermo Fisher Scientific) in Matrigel in 3D. Cultures were maintained at 37 C in a 5% CO 2 /5%O 2 atmosphere in a Galaxy 170R incubator (New Brunswick, Eppendorf).
Protein extraction and western blot analysis 3D cultured primary mammary cells were released from Matrigel using the BD cell recovery solution and lysed in Laemmli buffer. Protein extracts were separated by SDS-PAGE, transferred to PVDF membranes (IPVH00010, Merck Millipore, Hertfordshire, UK) and immunoblotted with antibodies detailed in the Key Resources Table. GAPDH or alpha-tubulin were used as loading controls. Resulting immunocomplexes were detected by HRP-conjugated anti-mouse IgG or anti-rabbit IgG secondary antibodies and enhanced chemiluminescent (ECL) reagents (WBLUF0100, Merck Millipore). Protein extracts (400 ug) from Ctr, BRCA1-, siCtrand siPin1-MDA-MB-468 cells were processed and analyzed for phosphorylation of LYN (Y397) and SRC (Y419) using the Human Phospho-Kinase Antibody Array (R&D Systems) following the manufacturer's instructions.

Immunoprecipitation (IP) LYN kinase assay
Once recovered from Matrigel, 3D cultured cells were lysed in RIPA buffer (50mM Tris/HCl, pH 7.5, 150mM NaCl, 1% Triton X-100, 1% Na deoxycolate, 0.1% SDS) supplemented with 1mM Na orthovanadate and protease inhibitor-cocktail (Roche, Burgess Hill, West Sussex, UK). After centrifugation (14000 g for 10 min at 4 C), supernatants (150 mg of protein per sample) were pre-cleared with protein A-Sepharose beads (GE Healthcare, Cardiff, UK) for 45 min at 4 C prior to incubation with anti-LYN antibodies (rabbit polyclonal sc-15) for 2 hr at 4 C. Immunocomplexes were pulled down after binding to protein A-Sepharose beads (GE Healthcare) for 45 min at 4 C and washed twice with 20 mM HEPES, pH 7.4, 5 mM MgCl2, 3 mM MnCl2 1mM, 1mM Na orthovanadate (kinase buffer). Beads were then resuspended in 50 mL of kinase buffer with 2.75 mg of acid denatured enolase (Sigma), 5-10 mCi of g 32 P ATP (PerkinElmer, Seer Green, Buckinghamshire, UK) and 1 mM cold ATP. After a 10 min-incubation at 30 C, the reaction was stopped by adding 13 mL of 10mM ATP, 50 mM EDTA and samples were subjected to SDS-PAGE on a 10% acrylamide gel. Gels were fixed in 10% methanol/ 10% acetic acid solution, then dried and developed by autoradiography. Intensities of bands corresponding to phosphorylated enolase were measured using the ImageJ software.

LYN-PIN1 co-immunoprecipitation
Primary BlgCre Brca1 fl/fl p53 +/À mouse tumor cells were collected in cold PBS pH 8.3 buffer with 10 mM EDTA, 0.1% Tween 20, 10 mM Sodium Fluoride, 1 mM Sodium Orthovanadate, 10 mM Sodium Pyrophosphate, 100 mM b-Glycerophosphate, 2 mM PMSF, complete Protease Inhibitors (Roche) and lysed by passing through a 26G needle. After centrifugation (14000 g for 15 min at 4 C), supernatants (3-4 mg of protein) were pre-cleared with protein A-Sepharose beads (GE Healthcare) for 45 min at 4 C prior to incubation with anti-Pin1 (rabbit polyclonal (H-123), sc-15340, Santa Cruz) or control (IgG) antibodies overnight at 4 C. After over 1min., held at 90%B for 6min and then reduced to 1%B over 1min.) with a flow rate of 300 nL min À1 . Solvent A was 0.1% formic acid and Solvent B was aqueous 80% acetonitrile in 0.1% formic acid. Peptides were ionized by nano-electrospray ionization at 2.0kV using a stainless steel emitter with an internal diameter of 30 mm (Thermo Scientific) and a capillary temperature of 275 C.
All spectra were acquired using an Orbitrap Fusion Tribrid mass spectrometer controlled by Xcalibur 2.0 software (Thermo Scientific) and operated in data-dependent acquisition mode using an SPS-MS3 workflow. FTMS1 spectra were collected at a resolution of 120 000, with an automatic gain control (AGC) target of 200 000 and a max injection time of 50ms. Precursors were filtered with an intensity threshold of 5000, according to charge state (to include charge states 2-7) and with monoisotopic precursor selection. Previously interrogated precursors were excluded using a dynamic window (60 s ± 10ppm). The MS2 precursors were isolated with a quadrupole mass filter set to a width of 1.2 m/z. ITMS2 spectra were collected with an AGC target of 10 000, max injection time of 70ms and CID collision energy of 35%.
For FTMS3 analysis, the Orbitrap was operated at 50 000 resolution with an AGC target of 50 000 and a max injection time of 105ms. Precursors were fragmented by high energy collision dissociation (HCD) at a normalized collision energy of 60% to ensure maximal TMT reporter ion yield. Synchronous Precursor Selection (SPS) was enabled to include up to 5 MS2 fragment ions in the FTMS3 scan.

TMT Data Analysis
The raw data files were processed and quantified using Proteome Discoverer software v2.1 (Thermo Scientific) and searched against the UniProt Human database (downloaded 14/09/17; 140000 sequences) plus LYNA and LYNB and LYNA_YF sequences using the SEQUEST algorithm. Peptide precursor mass tolerance was set at 10ppm, and MS/MS tolerance was set at 0.6Da. Search criteria included oxidation of methionine (+15.9949) as a variable modification and carbamidomethylation of cysteine (+57.0214) and the addition of the TMT mass tag (+229.163) to peptide N-termini and lysine as fixed modifications. Searches were performed with full tryptic digestion and a maximum of 2 missed cleavages were allowed. The reverse database search option was enabled and the data were filtered to satisfy false discovery rate (FDR) of 5%.

QUANTIFICATION AND STATISTICAL ANALYSIS
Unless otherwise stated, blots shown are representative of three independent experiments. Unless otherwise stated, all quantitation is shown as mean and SD from three independent experiments and statistical significance determined using two-tailed unpaired t tests. Gene expression analysis by quantitative real-time rtPCR is shown as mean ± 95% confidence intervals from three independent experiments, each of which was carried out using three technical replicates. Significance of real-time RT-PCR data was determined from confidence intervals (Cumming et al., 2007). *p < 0.05; **p < 0.01; ***p < 0.001.
Statistical analysis of tumor growth was conducted using the glmer function for generalized linear mixed models from the lme4 package (Bates et al., 2015) in the R software (version 3.2.2). The final model accounted for the change in tumor VOLUME with time (DAY) and a DAY-by-TREATMENT interaction as fixed effects using variable random intercepts and slopes for each tumor (TUMOUR_ID). This relationship was specified as glmer (VOLUME $ DAY + DAY:TREATMENT + (DAYjfTUMOUR_ID), family = Gaussian (link = ''log). All modelling assumptions were confirmed to be reasonable on diagnostic residual plots.
Number of phospho-H3-positive cells in FFPE sections of grafted tumors was determined by using ImageJ image analysis software (https://imagej.nih.gov/ij/). Automatic counting was performed on binary images (8-12 fields per tumor) after applying consecutive dilations to coalesce multiple dots within the same cell.
Band intensities on gels and western blots were also quantified using ImageJ.