Plasma genotyping identifies potentially actionable mutations at variable mutant allele frequencies, often admixed with multiple subclonal variants, highlighting the need for their clinical and functional validation. We prospectively monitored plasma genotypes in 143 women with endocrine-resistant metastatic breast cancer (MBC), identifying multiple novel mutations including HER2 mutations (8.4%), albeit at different frequencies highlighting clinical heterogeneity. To evaluate functional significance, we established ex vivo culture from circulating tumor cells (CTCs) from a patient with HER2-mutant MBC, which revealed resistance to multiple targeted therapies including endocrine and CDK 4/6 inhibitors, but high sensitivity to neratinib (IC50: 0.018 μM). Immunoblotting analysis of the HER2-mutant CTC culture line revealed high levels of HER2 expression at baseline were suppressed by neratinib, which also abrogated downstream signaling, highlighting oncogenic dependency with HER2 mutation. Furthermore, treatment of an index patient with HER2-mutant MBC with the irreversible HER2 inhibitor neratinib resulted in significant clinical response, with complete molecular resolution of two distinct clonal HER2 mutations, with persistence of other passenger subclones, confirming HER2 alteration as a driver mutation. Thus, driver HER2 mutant alleles that emerge during blood-based monitoring of endocrine-resistant MBC confer novel therapeutic vulnerability, and ex vivo expansion of viable CTCs from the blood circulation may broadly complement plasma-based mutational analysis in MBC.
The treatment of HR+/HER2− breast cancer has markedly evolved with the advent of multiple effective endocrine-based therapies, leading to significantly improved survival in women with metastatic breast cancer (MBC).1 Recently demonstrated clinical benefit from combining endocrine therapy with CDK 4/6 inhibitors led to approval of palbociclib (2015), ribociclib (2017), and abemaciclib (2018) as first-line therapies for patients with advanced HR+ breast cancer.2,3,4 However, endocrine resistance ultimately emerges, driven in part by the acquisition of activating mutations in the estrogen receptor (ER) gene ESR1 mediating resistance to aromatase inhibitors,5,6,7,8,9,10 but other mechanisms governing endocrine resistance are not well understood.
Tumor sampling to identify and monitor the presence of actionable drug resistance-associated mutations is a central tenet of targeted precision oncology. In chronic myeloid leukemia, resequencing of the BCR-ABL oncogene may direct use of second line inhibitors,11 while in lung cancer, repeat tumor biopsies may identify second site mutations within the driving EGFR and EML4-ALK oncogenes, or therapeutically actionable alterations in other genes capable of bypassing the inhibited cellular signaling, such as c-MET amplification.12 On-treatment tumor sampling in HR+ breast cancer, however, has been limited because many patients harbor only bone metastases, which are not readily amenable to biopsy. This together with many resistance-associated mutations in MBC not being druggable result in largely empiric therapeutic regimens for women with metastatic HR+ breast cancer.1
Blood-based monitoring is emerging as a robust tool to quantify tumor burden and assess response in patients with solid tumor malignancies, as well as to evaluate the evolution of tumor cell subpopulations, as they decrease or increase in response to therapeutic challenge.13,14,15 Plasma-based genotyping can integrate mutant allele fractions (MAFs) from multiple sites of metastatic disease, identifying distinct clonal derivatives that may have different drug sensitivity and resistance profiles. Indeed, given its ease of application, plasma-based mutation detection has rapidly gained popularity in the clinical setting. However, such plasma-based mutational data alone may not predict drug susceptibility, particularly when multiple mutations are simultaneously present at variable MAFs. In this context, functional validation for identification of driver alterations is critical. The isolation of viable tumor cells (CTCs) from the blood circulation and their expansion in vitro may complement ctDNA mutational analysis, enabling direct testing of drug effects on cell viability and cellular signaling.5 Ultimately, correlating clinical response to blood-based parameters is essential to rational treatment decisions. Here, we describe the frequent occurrence of HER2 mutations, which emerge in patients receiving endocrine-based therapy for HR+ MBC, and utilize patient-derived ex vivo circulating tumor cell (CTC) cultures to demonstrate that such mutations are functional drivers susceptible to novel targeted inhibition.
Detection of HER2 mutations by plasma-based genotyping in HR+/HER2− MBC
We prospectively collected plasma specimens from women with HR+/HER2− MBC who had disease progression on prior endocrine-based regimen, including CDK 4/6 inhibitors (N = 143). The blood samples were collected at the time of disease progression, prior to initiation of a second line or subsequent regimen (see Table 1 for detailed clinical characteristics of the cohort, including age at metastatic diagnosis; prior endocrine therapy including aromatase inhibitor, CDK4/6 inhibitors; timing of metastasis; and number of prior therapies). Plasma samples were analyzed by ctDNA genotyping, using a CLIA certified next generation sequencing (NGS)-based clinical assay (Guardant), which includes MAFs for a panel of 73 breast cancer associated genes (Supplementary Table 1).16 A total of 14 mutant alleles (11 unique mutations) were identified in 12 of the 143 patients (8.4%). Compared with all patients in the cohort, those with HER2 mutations had no distinguishing clinical characteristics, including age at diagnosis of metastatic disease, diagnosis as metastatic recurrence versus de novo metastatic disease, presence of visceral versus bone-only metastases, or prior adjuvant treatment including aromatase inhibitors (Table 1).
Of the eleven unique HER2 mutations, eight (72.8%) have been previously reported in cancer, while three (27.2%) are novel variants: L11R, F889I, and G1015A. While the functional significance of these novel variants is uncertain, we note that they are located within evolutionary conserved residues: F889I and G1015A affect amino acids that are conserved in all four species analyzed (human, pig, mouse, and rat), while L11R is conserved in human and pig. All together, the HER2 mutations span multiple domains, as depicted in Fig. 1a. Of the eleven unique mutations, most are in the tyrosine kinase domain (N = 6 unique mutations, accounting for nine mutant alleles), while others are in the extracellular domain (N = 4) and cytoplasmic tail (N = 1), consistent with different mechanisms implicated in the activation of this ligand-independent receptor. Most importantly, for eight cases, matched primary tumor specimens were available. However, the HER2 mutations were detectable in none of these, suggesting that they likely emerged under therapeutic pressure during the course of endocrine-based therapy (Table 2).
Two patients, Patient 1 and Patient 8, had two distinct HER2 mutations simultaneously detected in ctDNA, suggesting the polyclonal nature of these mutations in patients with MBC (Fig. 1b). MAFs for all HER2 mutations ranged from 0.1% to 19.8% (Table 2). Besides the HER2 mutations, multiple coexisting mutations were detected, albeit at different MAFs, highlighting clonal heterogeneity. Common coexisting mutations included ESR1 (41.6%), TP53 (25%), and PIK3CA (33.3%), all of which have been reported in endocrine resistant breast cancer.17 Interestingly, half the PIK3CA mutations were also present in the patients’ pretreatment metastatic tumor biopsies, which suggests these were possibly pre-existing truncal mutations (i.e. dominant mutations shared by subsequent clones). The pre-existing PIK3CA mutations were H1047R and E545K, both known hotspot mutations, and in subsequent ctDNA sampling the former remained the dominant mutation (59%), and the latter in a percentage comparable to the accompanying mutations (0.3%). One patient (12, Table 2) also appeared to have acquired a small percentage PIK3CA mutation E722D, though the quantity was comparatively low (0.3%), and this is not a known hotspot mutation. In contrast, the activating ESR1 mutations, like the HER2 mutations, were detected only in the posttreatment ctDNA sample, indicating acquired selection during drug therapy. The TP53 mutations in ctDNA were also not detected in the tissue biopsy, although there is incomplete overlap in the specific TP53 mutations detected by the tumor versus ctDNA assays. Of note, within individual patients, HER2 and ESR1 subclonal mutations appeared at different allele frequencies, raising the possibility that these two distinct resistance mechanisms contribute toward the full complement of drug resistance in heterogeneous tumor populations (Table 2).
Analysis of patient-derived ex vivo cultured CTCs with HER2 mutation
To provide functional validation for the HER2 mutations detected by plasma genotyping, we analyzed viable CTCs that were successfully expanded in vitro from a subset of patients in the cohort. We used a microfluidic “negative depletion” CTC-iChip platform5,18,19 to process 10 ml of whole blood, effectively removing normal hematopoietic cells and enriching for unmanipulated viable CTCs. CTCs were successfully cultured from Patient 2 (Fig. 1a) who had a HER2 S310F mutation identified by ctDNA genotyping, and the HER2 mutation was confirmed in the CTC-derived cultures.
The clinical therapeutic history and timing of CTCs cultured from Patient 2 (Fig. 1a; BRx140) are shown in Fig. 2a, along with a comparable CTC culture from a patient (BRx50) with wild-type HER2.5 The corresponding CTC cultures are illustrated in Fig. 2b. A heterozygous HER2 mutation (S310F) is evident in BRx140 cells, identical to the mutation identified in the ctDNA from Patient 2 (Fig. 2c). This mutation was not detected in a tumor infiltrated lymph node resected prior to the development of endocrine drug resistance, consistent with an acquired genetic event. Patient characteristics and additional mutations scored in HER2-mutant CTC cell line (BRx140) and HER2-wild-type CTC cell line (BRx50) are described in Supplementary Table 1A and B. The patient-derived CTC cell line BRx140 provided a robust tool for us to study functional properties of mutant HER2, compared to the BRx50 CTCs, which are wild type for HER2, but harbor an ESR1 mutation5 (Supplementary Fig. 1A).
Treatment of the cultured CTCs with the ER degrader fulvestrant, the ER modulator tamoxifen, or the CDK4/6 inhibitors, palbociclib or ribociclib, showed no difference between cells harboring or lacking a HER2 mutation (Supplementary Fig. 1B). The relative insensitivity of these cultured CTCs to these agents is consistent with the cases of hormone-refractory breast cancers from which they were derived (Supplementary Fig. 1B). In contrast, HER2-mutant CTCs (BRx140) were highly sensitive to treatment with the HER2 inhibitor neratinib (IC50: 0.018 μM) and moderately sensitive to lapatinib treatment (IC50: 0.0837 μM), whereas CTCs with wild-type HER2 (BRx50) were resistant to both neratinib (IC50: 1.151 μM) and lapatinib (IC50: 9.603 μM) (Fig. 3a–d).
Immunoblotting analysis of the HER2-mutant BRx140 CTCs showed high levels of HER2 expression at baseline, which was suppressed by neratinib exposure, consistent with its known effect on receptor internalization and degradation.20 No such effect was seen in the BRx50 cells with wild-type HER2 expression. Remarkably, phosphorylation of the downstream signaling effectors S6 and ERK was abrogated following treatment of HER2-mutant CTCs with neratinib (Fig. 3e), indicating that signaling by mutant HER2 is the primary driver of proliferative signals in these cells. In contrast, phospho-S6 and phospho-ERK levels in the HER2-wild-type CTCs (BRx50) were unaffected by neratinib, consistent with the presence of alternative drivers of cellular proliferation. Thus, functional studies of HER2 targeting in CTC-derived cultures from a patient who had acquired a HER2 mutation during the course of endocrine therapy suggests that the emergence of this mutation may drive a new oncogenic dependency that is susceptible to therapeutic intervention.
Therapeutic response in a patient with ctDNA positive for two HER2 mutations
To evaluate therapeutic inhibition, we evaluated the treatment patterns. In this cohort, three patients with HER2 mutant alleles identified by ctDNA genotyping were treated with neratinib, an irreversible, pan-HER kinase inhibitor. One patient (index Patient 1 in Fig. 1b) had two coexisting HER2 mutations (S310Y and G727A) and two activating ESR1 mutations (D538G and E380Q) based on plasma genotyping and had adequate follow-up for determination of treatment efficacy. Of the two other patients with HER2 mutant alleles who received neratinib, one had rapid disease progression before receiving neratinib (off-label compassionate use) and could only receive a few doses before discontinuation of all medical therapies and enrollment in hospice care, and the other recently started treatment and has not yet received the required follow-up for evaluation of treatment efficacy. The other nine patients received different therapies, consistent with the availability of multiple treatment options for MBC (data-cut off September 30, 2018).
The index patient is noteworthy for having received multiple prior endocrine therapies, including aromatase inhibitor and SERD, for HR+/HER2− MBC (Fig. 4a). She was treated with neratinib and fulvestrant, as part of an IRB-approved basket clinical trial, resulting in a significant reduction in tumor volume (37% reduction per RECIST at 10 months; Fig. 4b). Repeat ctDNA analysis using the same assay after 6 months of treatment showed a complete molecular response, with disappearance of both HER2 mutations. Interestingly, while the HER2 mutant alleles targeted by neratinib rapidly resolved, the pharmacodynamic effect of fulvestrant on ESR1 mutant alleles appeared to be more modest. The E380Q ESR1 mutations, which had a very low MAF, resolved, but the more abundant D538G ESR1 mutation was only partially reduced. The MAF of other mutations, including NF1 and EGFR mutations, was unaffected by the neratinib and fulvestrant combination therapy (Fig. 4c).
The absolute level of MAF for different mutations and their rate of change as a function of therapy allowed modeling of tumor subpopulations in this patient, suggesting four dominant clones: a major tumor cell population harboring HER2 G727A, which declined rapidly on-treatment; a second population harboring ESR1 D538G, which declined slowly, but within which a smaller fraction with HER2 S310Y disappeared rapidly on-treatment; a third subpopulation with EGFR V536M, a fraction of which also had NF1 Y489C, which remained stable on-treatment; and a fourth minor subpopulation with a ESR1 mutation E380Q, which became undetectable on-treatment (Fig. 4d). Thus, three of the four identified tumor subpopulations harbored four different resistance alleles, with the HER2 mutations displaying prompt response to neratinib, while the ESR1 mutations appeared to decline more modestly following fulvestrant. The total ctDNA tumor burden was reduced (total MAF from 3.9% to 2.3%), consistent with the presence of a subset of tumor cells harboring HER2 mutations and reflecting the partial clinical response observed in the patient.
In this translational study, we demonstrate the emergence of HER2 mutations, detectable by plasma DNA sequencing, in women with HR+/HER2− MBC who have developed clinical resistance to endocrine-based combination therapies, and provide functional validation based on patient-derived CTC culture models. Acquired mutations in the setting of clinical progression often arise along with mutations in other genes, and may be present as dominant clones, or less prevalent subclones. It is in this context that functional studies are required to demonstrate the physiological significance of these acquired mutations as “drivers” of proliferation, rather than incidental passengers. We provide two lines of evidence to support the clinical importance of the HER2 mutations: first, in one patient treated with the HER2 inhibitor neratinib who was evaluable for response, the two subclonal HER2 mutations disappeared within 6 months of treatment initiation, whereas other concurrent mutations, marking other HER2-wild-type subclones, were not changed. The patient remained in prolonged partial remission for >1 year. Second, using ex vivo cultured CTCs from a patient with an acquired HER2 mutation, we demonstrate that, in these but not in HER2-wild-type CTCs, neratinib abrogates the major downstream signaling pathways for cell survival and proliferation, an effect that is associated with exquisite sensitivity of the cultured CTCs to HER2 inhibition. Together, these observations point to the emergence of HER2 mutations as a recurrent mechanism of disease progression in HR+, HER2− breast cancer, and suggest that this mechanism of clinical resistance to endocrine therapy may be associated with de novo sensitivity to HER2 inhibition in some patients.
Activating mutations in HER2 have been reported in small subsets of multiple different cancers.21,22,23,24 In primary breast cancer, they are particularly rare, with an estimated prevalence of 1.8% in primary tumors based on The Cancer Genome Atlas analysis.25 While this manuscript was in preparation, another group reported a high prevalence of HER2 mutations (6%) based on tissue genotyping of metastatic specimens in endocrine-resistant HR+/HER2− breast cancer,26 and two groups demonstrated enrichment of HER2 mutations in ctDNA after treatment with endocrine-based therapy.27,28 As in these studies, we cannot determine whether these mutations were present below detection at the time of diagnosis and were subsequently enriched during the course of endocrine therapy, or whether they were completely absent from the original tumor but arose through de novo mutation during cancer progression. In our study, none of the eight ctDNA-positive patients for whom primary tumor material was available for sequencing had evidence of detectable HER2 mutant alleles within the archival tissue specimen (<0.1% MAF). Interestingly, none of the HER2 mutant cases had identifiable metastatic disease at presentation, thus it is unlikely these mutations arose within a specific metastatic tumor lesion that had not received prior endocrine-based therapy. Future studies would benefit from collecting plasma ctDNA at the time of diagnosis to confirm the presence or absence of mutations. In addition, detailed information about certain clinical characteristics, such as disease-free interval (from early stage to metastatic) and histology (lobular versus ductal), was not available in the database and the study observations require validation in additional studies.
Unlike the prototypical HER2 gene amplifications that define a major subset of primary breast cancer and are highly correlated with response to HER2-targeting antibodies, point mutations in HER2 are less well characterized, and their occurrence within multiple domains of the receptor, including extracellular, catalytic, and cytoplasmic tail, make them less readily interpretable than recurrent kinase domain mutations, such as observed in the related receptor EGFR.29
Moreover, unlike HER2-amplified breast cancer, tumors harboring HER2 mutations appear to be resistant to standard HER2-targeted antibodies, including trastuzumab.23 HER2-mutant breast cancers exhibit mixed responses to the most commonly used small molecular inhibitor, lapatinib, although they may be more sensitive to more potent irreversible HER2 inhibitors, such as neratinib.23,30 Lapatinib and neratinib were chosen to test the response to reversible and irreversible HER2 inhibition, respectively, utilizing two drugs that are FDA approved. The clinical efficacy of neratinib in metastatic HER2 mutant solid tumors, including breast cancer, was recently described in a landmark “basket” trial.31 In the study by Hyman et al., an objective response rate of 32% (95% CI: 15–54%) was noted in patients with HER2-mutant breast cancer (N = 25), with responsive tumors having mutations in extracellular domains as well as the tyrosine kinase domain. Variable clinical responses were also reported with neratinib in a trial of HER2-mutant MBC, screened by tissue-based genotyping.32 Together with our own study, these results extend the therapeutic application of HER2 targeted therapies to HER2 mutations that emerge after endocrine-based therapy and are identified at various allele frequencies coexisting with other mutations. The prevalence of HER2 mutations appears to be considerably higher in these patients, who received endocrine therapies with or without CDK4/6 inhibitors, compared with the HER2 mutation frequency established in untreated primary breast cancer.
Oncogene addiction by cancer cells was classically defined as resulting from their inherent wiring through a dominant or “truncal” mutation that drives oncogenic signaling in the cell.33 As such, it is uncertain whether mutations acquired during the course of cancer progression may mediate similar dependencies, particularly if they constitute subclonal late somatic events that arise in the context of multiple other mutations. Indeed, most HER2 mutations have been functionally annotated using ectopic expression in preclinical model, which cannot predict their oncogenic dependence when arising endogenously in cancer cells.34 The difficulty in assessing the clinical relevance of acquired HER2 mutations is all the more critical with the advent of liquid biopsies, which may identify large numbers of potentially actionable mutations present at low allele frequencies. For example, besides HER2 mutations we also observed ARID1A mutations that suggests emergence of epigenetic escape or adaptive response mechanisms, requiring further evaluation in additional studies. While larger data sets will be required to confirm our observations, the data presented here suggests that even at subclonal allele frequencies, the acquisition of HER2 mutations denotes a potential therapeutic opportunity. These data are supported by recently published research identifying activating mutations in HR+ breast cancer, which similarly appears to confer resistance to hormonal therapy, but sensitivity to neratinib.35 Similarly, this study describes mutations found in a relatively small population, eight patients, thus our work compliments these findings and supports the principle of acquired activating mutations conferring both endocrine resistance, as well as a new sensitivity to HER2-targeted therapy. As such, HER2 mutations join ESR1 mutations as recurrent mechanisms of acquired resistance to endocrine combination therapy, which may coexist within individual patients, and both of which have potentially important therapeutic implications.
Plasma ctDNA analysis has previously been used to track the emergence of activating mutations in ESR1, which are common in women treated with aromatase inhibitors.10 The distinct tracking of HER2 and ESR1 ctDNA mutations in our index patient responding to combined neratinib and fulvestrant therapy is consistent with the presence of multiple coexisting tumor subpopulations, each responding with unique dynamics. The diverse clonal nature of endocrine drug resistance is exemplified by patient-derived cultured CTCs exhibiting one or the other mechanism. Treatment options in patients who harbor multiple subclonal mechanisms of endocrine drug resistance are not established and may require ongoing assessment of dominant clones following treatment interventions. We note, however, that the sustained response in our index patient is correlated with the dramatic decline in HER2 MAF, with a more modest response to ER targeting fulvestrant, raising the possibility that HER2-activated tumor clones may contribute disproportionately to tumor proliferation and expansion in this patient.
In summary, the emerging use of ctDNA genotyping to monitor response and potentially guide therapeutic choices brings with it the challenge of evaluating the predictive and functional value of multiple subclonal mutant alleles as potentially therapeutic targets. The fact that acquired oncogenic driver mutations may mediate resistance to an initial therapeutic regimen, while establishing sensitivity to a second treatment option highlights new opportunities in precision targeting of acquired mutations to prolong clinical responses for patients with MBC.
Patient selection and genomic analysis
Blood specimens were collected after informed consent as either standard of care for clinical genotyping or under an IRB approved tissue/blood collection protocol from patients with histologically confirmed HR+/HER2− MBC at the Massachusetts General Hospital and underwent ctDNA testing utilizing a CLIA certified ctDNA assay (Guardant), an NGS-based commercially available assay that detects ctDNA down to 0.1% allelic fraction with a clinical sensitivity of 85% (compared to 80.7% in tissue) and 99.8% specificity.16 We also reviewed the genomic profile results of the matched patient-derived primary or metastatic tumor biopsies, and the CTC cultures utilizing the SNaPshot-NGS clinical assay, an institutional anchored multiplex PCR assay that detects SNVs and indels in tissue biopsies. Independent chart review was utilized to gather data on clinico-pathological characteristics, mutation data (from Guardant clinical reports and Snapshot clinical reports), and clinical outcomes.
Statistical significance was defined as P < 0.05. Stata (StataCorp. 2015. Stata Statistical Software: Release 14. College Station, TX: StataCorp LP) was used to perform analyses.
Enrichment of patient CTCs
Informed consent (written) was obtained from MBC patients for CTC collection as per Dana Farber/Harvard Cancer Center institutional review board approved protocol (DF/HCC 05–300). Twenty millilitres of whole blood was obtained from BRx140 in two EDTA tubes and CTCs were isolated using the microfluidic CTC-iChip as previously described.19 In brief, whole blood was incubated with biotinylated antibodies against CD45 (clone 2D1; R&D Systems), CD66b (clone 80H3; AbD Serotec), and CD16 (Janssen Diagnostics) followed by incubation with Dynabeads MyOne Streptavidin T1 (Invitrogen) to achieve magnetic labeling of leukocytes. This blood was then processed through the CTC-iChip and the product was collected in CTC culture media (see below) under aseptic conditions for derivation of patient-specific CTC cultures.
Ex vivo CTC culture
CTC cultures were grown in CTC media comprising of RPMI-1640, bFGF (20 ng/ml), EGF (20 ng/ml), 1X B27, and 1X antibiotic/antimycotic (Life Technologies) in ultralow attachment flasks (Corning) at 37 °C under hypoxic conditions (4% O2) with 5% CO2. Cultures were routinely checked for mycoplasma with the MycoAlert and Lonza Kit and tested for authentication via STR profiling by Genetica DNA Laboratories (a LabCorp brand; Burlington, NC) using the commercially available PowerPlex® 16HS amplification kit (Promega Corporation; mouse marker included) and GeneMapper ID v3.2.1 software (Applied Biosystems). The CTC line BRx 50 has been previously described.5
A total of 100 nM of Neratinib was added to 5 × 105 cells for 24 h and 10 μg each of protein lysates were separated on SDS/4–15% polyacrylamide gels (Bio-Rad) and transferred onto nitrocellulose membranes (Invitrogen). The blots were incubated with antibodies directed against GAPDH [(14C10) cell signaling #2218], HER2 [(29D8) cell signaling #2165], Erk1/2 [cell signaling #9102], Phospho-Erk1/2 [(Thr202/Tyr204) cell signaling #9101], phospho-S6 ribosomal protein [(Ser235/236) cell signaling #2211], and S6 ribosomal protein [(5G10) cell signaling #2217] and with the relevant secondary antibodies and visualized using Odyssey Clx (LI-COR). All blots were derived from the same experiment and were processed in parallel. In Supplementary Material, all blots and gels are accompanied by the locations of molecular weight/size markers and uncropped scans (Supplementary Fig. 2).
Dose response curves for drug sensitivities
A total of 1000 cells were seeded in a 96-well ultra-low attachment plate (Corning). Increasing concentrations of neratinib (HKI-272) (Selleckchem S2150), lapatinib (Selleckchem S2111), tamoxifen (Selleckchem S1238), and fulvestrant (Selleckchem S1191) were added to quadruplicate samples. The cells were incubated with the above drugs for 5 days under hypoxic conditions. Viability was measured using CellTiter-Glo Luminescent Cell Viability Assay per the manufacturer’s instructions.
CDK4/6 inhibitor treatment
A total of 2000 cells were seeded in a 96-well ultralow attachment plate (Corning). A total of 500 nM ribociclib (LEE011) (Selleckchem S7440) and 500 nM palbociclib (PD-0332991) HCl (Selleckchem S1116) were added to quadruplicate samples for 3 days and viability was measured using CellTiter-Glo Luminescent Cell Viability Assay per the manufacturer’s instructions.
DNA extraction, PCR, and sanger sequencing
DNA was extracted using All Prep DNA/RNA Mini Kit from Qiagen per the manufacturer’s instruction. PCR was performed with 100 ng of DNA and primers flanking the mutation using KAPA HiFi HotStart ReadyMix PCR Kit based on the manufacturer’s instructions. PCR products were purified using QIAquick PCR Purification Kit from Qiagen followed by Sanger sequencing by Eton Bioscience Inc.
ESR1 forward primer: 5′-TGGAAGTCACCTGCATAGCAAATACCCTG-3′
ESR1 reverse primer: 5′-GCAAATGAATGGCCACTCATCTAGAAAGCC-3′
HER2 forward primer: 5′-TAACAGATCACCTATTTACTGATGGGC-3′
HER2 reverse primer: 5′-CACTGACAGGGGATATAGGGACACTTGTA-3′
Data availability statement
Sequencing data submitted to GenBankBank, accession code: MN047439, MN047440, MN047441, and MN047442. Additional data available on request from the authors.
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We thank all the patients who participated in this study. We are grateful to Massachusetts General Hospital (MGH) nurses for their help with the study; and L. Libby for invaluable technical support. This work was supported by the NIH Grant R01CA129933, the Breast Cancer Research Foundation, the Howard Hughes Medical Institute, and the National Foundation for Cancer Research (to D.A.H.), the NIH Quantum Grant 2U01EB012493 (to D.A.H.), the NIH Grant U01CA214297 (to D.A.H and S.M), the ESSCO Breast Cancer Research (to S.M.), the Susan G Komen Grant CCR15224703 (to A.B), K12 5K12CA087723 (to A.B.), KL2 TR001100 (to L.M.S), and the ASCO Young Investigator Award (to L.M.S).
MGH has filed for patent protection for the CTC-iChip technology. D.J. has served as a Consultant/Advisory Board at Novartis, Genentech, Eisai, Ipsen, and EMD Serono. L.S. has served as a Consultant/Advisory Board at Novartis. S.I. has served as a Consultant/Advisory Board at Abbvie, PharaMar, Genentech/Roche, Myriad Genetics, Hengrui Therapeutics, Puma Biotech, and Immunomedics. B.M. spouse has served as a Consultant/Advisory Board at MOTUS GI. A.J.I has served as a Consultant/Advisory Board at Roche, Chugai, Constellation, and Pfizer, and has ownership interests and intellectual property rights/inventor/patent holder at ArcherDx. A.B. has served as a Consultant/Advisory Board at Novartis, Pfizer, Genentech/Roche, Radius Health, Merck, Spectrum pharma, Immunomedics, Sanofi, Daiichi Pharma, and Taiho Oncology, and has research Grant from Biothernostics (self), Genentech (institution), Novartis (institution), Pfizer (institution), Merck (institution), Sanofi (institution), Radius Health (institution), Immunomedics (institution), Mersana(institution), and Innocrin (institution). All other authors declare no competing interests.
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Medford, A.J., Dubash, T.D., Juric, D. et al. Blood-based monitoring identifies acquired and targetable driver HER2 mutations in endocrine-resistant metastatic breast cancer. npj Precis. Onc. 3, 18 (2019). https://doi.org/10.1038/s41698-019-0090-5
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