Abstract
Utility of PI3Kα inhibitors like BYL719 is limited by the acquisition of genetic and non-genetic mechanisms of resistance which cause disease recurrence. Several combination therapies based on PI3K inhibition have been proposed, but a way to systematically prioritize them for breast cancer treatment is still missing. By integrating published and in-house studies, we have developed in silico models that quantitatively capture dynamics of PI3K signaling at the network-level under a BYL719-sensitive versus BYL719 resistant-cell state. Computational predictions show that signal rewiring to alternative components of the PI3K pathway promote resistance to BYL719 and identify PDK1 as the most effective co-target with PI3Kα rescuing sensitivity of resistant cells to BYL719. To explore whether PI3K pathway-independent mechanisms further contribute to BYL719 resistance, we performed phosphoproteomics and found that selection of high levels of the cell cycle regulator p21 unexpectedly promoted drug resistance in T47D cells. Functionally, high p21 levels favored repair of BYL719-induced DNA damage and bypass of the associated cellular senescence. Importantly, targeted inhibition of the check-point inhibitor CHK1 with MK-8776 effectively caused death of p21-high T47D cells, thus establishing a new vulnerability of BYL719-resistant breast cancer cells. Together, our integrated studies uncover hidden molecular mediators causing resistance to PI3Kα inhibition and provide a framework to prioritize combination therapies for PI3K-mutant breast cancer.
Similar content being viewed by others
Introduction
Cancer complexities undermine efficacy of anti-cancer treatments, but identification of cellular and molecular contexts provides opportunities for more effective therapies. PIK3CA encodes the p110α subunit of PI3K and is mutated in ~40% of luminal, estrogen receptor positive (ER+) breast cancer1. PI3K phosphorylates PIP2 and generates PIP3, which activates several effector targets to sustain cellular growth. The 3-phosphoinositide-dependent protein kinase 1, PDK1 and AKT are critical mediators of the PI3K signaling output. PDK1 phosphorylates AKT on T308, and a second phosphorylation event catalyzed by the mTOR complex 2 (mTORC2) on AKT S473, leads to full AKT activation and promotion of cell growth and proliferation (Fig. 1a)2.
Numerous drug agents have been developed to inhibit PI3K pathway components for cancer treatment3. The PI3Kα inhibitor alpelisib, i.e., BYL719, has been approved for the treatment of PIK3CA-mutant, ER+ metastatic breast cancer and is in clinical testing for additional malignancies4. However, PI3Kα inhibitors in monotherapy fail to induce stable tumor remission due to a number of factors, including dynamic reactivation of growth-promoting signaling nodes which cause treatment failure5. Acquisition of secondary mutations in compensatory genes also contributes to resistance to PI3Kα inhibition6, highlighting the urgent need to identify co-targets that complement single PI3Kα-targeting agents.
To this end, studies have found that several markers of resistance to PI3Kα inhibition are linked to reactivation of members of the PI3K pathway. These include mTORC17,8, p110β9, and activation of the PDK1-SGK1 axis10. Inhibition of the Retinoblastoma tumor suppressor, Rb, via selection of high levels of cyclin D1, was also reported to cause resistance to BYL71911, indicating that cell cycle regulators play a critical role in moderating cellular responses to this drug.
The discovery of various mechanisms of resistance to PI3Kα inhibition in recent years has led to the development of combination therapies that rescue the sensitivity to BYL719 in pre-clinical models of breast cancer5. However, the wealth of combinatorial treatments for BYL719-resistant breast cancer also raises the challenge of how to best prioritize the application of these new targeted therapies to improve patients’ outcomes. Moreover, whether additional PI3K pathway-independent mechanisms contribute to the resistance to PI3K-based therapies in breast cancer has not been fully explored.
By integrating previously identified mechanisms causing resistance to BYL719, we have constructed quantitative and predictive mathematical models representing the PI3K signaling network under a BYL719-sensitive versus BYL719-resistant cell state. Using in silico modeling, we tested how targeted inhibition of each member of the PI3K network synergized with PI3Kα inhibition, and the effect this combination would have on cell proliferation. We found that PDK1 was the top predicted co-target with PI3Kα suppressing activation of critical biomarkers of resistance and enhancing response to BYL719 in parental and BYL719-resistant T47D cells. Through phosphoproteomics we also found that control of DNA damage response pathways by the cyclin-dependent kinase (CDK) inhibitor p21 hides an unexpected vulnerability of BYL719-resistant cells. Consistently, targeting the Checkpoint kinase 1, CHK1, specifically caused death of BYL719-resistant T47D cells. Altogether, these studies reveal the contribution of unappreciated markers of resistance to PI3Kα inhibition, and provide an integrated framework that can be exploited for the identification of more tailored treatments for breast cancer patients.
Results
Integrated computational models capture signal dynamics of PI3K network
To provide a systems-level understanding of signaling dynamics occurring upon drug perturbations, including PI3Kα inhibition, we developed a mechanistic computational model that captures the complexity of the PI3K signaling network. The model was formulated using ordinary differential equations (ODEs) describing biochemical interactions as a series of ODEs based on established kinetic laws12. The model integrates canonical components of the PI3K pathway and contains reported signaling hubs implicated in the acquired resistance to BYL719 (Fig. 1a). These include: p110α and β-isoforms of PI3K and key downstream effectors (AKT/mTOR/S6K1, SGK3/NDRG1, SGK1/FOXO3, P-Rex1/Rac1, c-Myc); parallel signaling cascades (PI3K/AKT/mTOR, Ras/Raf/MEK/ERK, ERα) and prominent receptor tyrosine kinases (RTKs) such as IGFR/IR and ErbB; nodes converging on critical cell cycle checkpoints (CDKs/Rb/Cyclin D/E and p21) (Fig. 1a). Importantly, the PI3K model also encapsulates feedback and feed-forward molecular loops together with reported crosstalk mechanisms: AKT/mTORC1/S6K1/IRS; AKT/FOXO3/ErbB; CyclinD/CDKs/TSC2/mTORC1. Description of model generation, model reactions, ODE equations, model scope and assumptions are included in Supplementary Information.
To provide context specificity to the in silico representation of the PI3K network, we calibrated our model against data obtained from the ER+, T47D human breast cancer cell line harboring the PIK3CA H1047R mutation, and sensitive to BYL71913. Model calibration involves estimation of unknown model parameters to minimize mismatch between experimental data and simulated outputs12,14. To perform this, we employed a combination of new kinetic and dose-response data together with published reports monitoring phosphorylation and total levels of multiple nodes of the PI3K network under distinct stimuli, IGF-1/Insulin and HRG (Fig. 1b and Supplementary Fig. 1A)15,16. Parameter estimation was implemented using a genetic algorithm-based optimization procedure coded in MATLAB (Supplementary Information). Given the large size of our model, we assumed that multiple parameters would likely fit the experimental data equally well, a phenomenon commonly known as “model unidentifiability”16. To mitigate potential biases of using a single best-fitted parameter set, and overcome model unidentifiability, we employed an ensemble approach whereby we repeated the parameter estimation process with different starting points of parameter values, and obtained multiple parameters sets (n = 77) that fitted the data with similar high quality. These parameters sets were collectively used for subsequent simulations (Supplementary Fig. 1B and Supplementary Dataset 1) and demonstrated a faithful replication of experimental data (Fig. 1b). We refer to this calibrated model the ‘parental PI3K model’ as it describes the state of the BYL719-sensitive, parental T47D cell line.
To independently validate the parental PI3K model, we generated new predictions and compared these to new experimental data. We simulated dynamic activation of multiple network proteins in T47D cells in response to growth-media stimulation over 24 h, with or without BYL719, and performed corresponding experiments for validation (Supplementary Fig. 1C, D). Simulations correctly predicted that inhibition of key signaling markers such as ERK, AKT, S6 and Rb would occur in T47D cells in response to BYL719 (Supplementary Fig. 1D). These iterative computational-experimental analyses allowed us to build a predictive model tailored to study signaling dynamics in T47D cells.
To generate a computational model that recapitulates a cell-state associated with resistance to PI3Kα inhibition, we established pools of BYL719-resistant T47D cells, i.e., Resistant Pools (RP) 1, RP2 and RP3 (Fig. 1c). We performed 2D and 3D growth assays and found that BYL719 had a potent cytostatic effect on parental cells while BYL719-RPs kept proliferating even under high BYL719 concentration, confirming their resistant behavior (Fig. 1c, d and Supplementary Fig. 1E, F). We then profiled phosphorylation and total levels of key components of the PI3K network in RPs and T47D parental cells under standard growing condition, and used these data to adjust the parental model and generate the ‘resistant PI3K model’ (Supplementary Fig. 2A, B and Supplementary Information). We further validated both models by generating predictions of temporal changes in phosphorylation levels of important molecular hubs (AKT, ERK and S6) upon BYL719 treatment. Model simulations showed rapid inactivation of these signaling molecules in parental and RPs upon drug treatment (Fig. 1e) but also predicted that levels of phospho-S6 would remain higher in RPs than parental T47D cells. Time-course characterization of phospho-AKT, phospho-ERK and phospho-S6 in response to BYL719 confirmed model predictions (Fig. 1f, g and Supplementary Fig. 2C, D) and was consistent with previous reports7,8.
Collectively, we conclude that our parental and resistant-PI3K models faithfully recapitulate signaling dynamics observed in BYL719-sensitive and resistant T47D cells and define new quantitative tools to explore signaling dynamics in defined molecular settings.
Computational modeling prioritizes synergism between drug combinations
To prioritize efficacy of combinatorial therapies for BYL719-resistant breast cancer, we exploited our computational models and simulated the effect of various pair-wise drug combinations directed at PI3Kα and other components of the PI3K network. We interrogated 24 network nodes and simulated the consequences of inhibiting each of them along with PI3Kα. To assess the efficacy of each drug combination, we used cyclin D1, Rb, and S6 as molecular readouts given their established role in promoting cell growth and resistance to BYL7197,8,11. Moreover, higher cyclin D1 levels and phospho-S6, and reduced Rb activity were found in our RPs compared to parental T47D cells (Supplementary Fig. 3A).
In silico simulations compared the effect of inhibiting either PI3Kα alone, one single PI3K network target, or PI3Kα plus a network target, and assessed the synergism of each pair-wise drug combination on cyclin D1 levels and phosphorylated Rb and S6 (Fig. 2a–f and Supplementary Fig. 3C, D). Possible synergistic effects (or lack thereof) were quantified using the coefficient of drug interaction (CDI) index where CDI < 1, =1, >1 indicate a synergistic, additive, or antagonistic effect, respectively17. Accordingly, CDI values allowed us to rank simulated drug combinations and prioritize the most synergistic pairs for experimental validation. We found strong consistency between predicted drug combinations ranking across the molecular readouts indicating robustness in model predictions (Supplementary Fig. 3B).
As previously indicated, our model simulations consistently found that co-targeting IGF1R8, members of the SGK family of kinases10, mTORC17 with BYL719, would reduce cyclin D1 levels, promote Rb reactivation, and also inhibit S6 phosphorylation in parental cells (Fig. 2a–c and Supplementary Fig. 3C) and RPs (Fig. 2d–f and Supplementary Fig. 3D), thus affecting the status of biomarkers of resistance to BYL719. Notably, the top predicted synergistic co-target with PI3Kα, for both parental and resistant model, was PDK1 (Fig. 2a–f). Time-course simulations showed that while single PI3Kα or PDK1 inhibition blocked major signaling markers (phospho-AKT, phospho-S6, and cyclin D1) to some extent (Fig. 2g), combined PI3Kα plus PDK1 inhibition markedly and durably inhibited these signals over 48 h of drug treatment (Fig. 2g). To validate this, we treated parental and RP cells with BYL719 and the PDK1 inhibitor GSK2334470, either in single or in combination, and measured the dynamic responses of phospho-Rb, Cyclin D1, phospho-AKT and phospho-S6 over 48 h (Fig. 2h). We found that BYL719 plus GSK2334470 suppressed these growth-promoting markers more potently than single-drug treatments, at 24 and 48 h (Fig. 2h and Supplementary Fig. 3E) thus demonstrating durable synergism. Importantly, BYL719 plus GSK2334470 significantly blocked growth of parental and BYL719-resistant cells (Fig. 2i) confirming the superior anti-proliferative effect.
Finally, to determine the suitability of PDK1 and PI3Kα as therapeutic co-targets, we explored genetic dependencies using the Cancer Dependency Map (DEPMAP) database17. We found that compared to cells with wild-type PIK3CA (n = 13), PIK3CA-mutant breast cancer cell lines (n = 7) displayed increased dependency on PDK1 and were more susceptible to PDK1 knock-out for their proliferative capacity (Supplementary Fig. 3F).
Together, these integrated computational and experimental analyses support the notion whereby co-targeting PI3Kα with PDK1 defines an optimal strategy to fully inhibit PI3K pathway in PIK3CA-mutant cells resistant to BYL719.
Selection of high p21 levels promotes resistance to PI3Kα inhibition
To explore whether additional signaling axes outside the PI3K network contribute to BYL719 resistance, we conducted quantitative mass spectrometry (MS)-based phosphoproteomics. Parental and RPs cells were processed according to the label-free quantitative MS method (Fig. 3a) and phospho-peptides quantified (Fig. 3b and Supplementary Fig. 4A). Enrichment of phospho-Ser/Thr and Tyr peptides allowed us to identify 8495 phospho-peptides and 6065 total peptides (Fig. 3b). Ingenuity Pathway Analysis (IPA)18 revealed that control of cell cycle checkpoints and response to DNA damage pathways were both highly enriched in RPs relative to parental, sensitive T47D cells (Fig. 3c). Consistently, cell cycle analysis by flow cytometry confirmed that BYL719 had a potent cytostatic effect on parental cells, which arrested in G0-G1 and G2-M phases, whereas RPs kept cycling and dividing irrespective of the inhibitor (Fig. 3d).
Next, we monitored activation status and expression level of key members of cell cycle checkpoints by Western Blotting (WB) (Fig. 3e). In addition to confirming high levels of cyclin D1 and phospho-Rb, we noticed that RPs showed an unexpected increase in the levels of the CDK inhibitor p21 compared to parental cells (Fig. 3e). These changes were accompanied by increases at the mRNA level, indicating a likely transcriptional regulation (Fig. 3f). Interestingly, this condition was unique to p21 as other CDK inhibitors (p27, p18 and p53) showed no alterations across cell lines (Fig. 3e). However, since T47D cells express a mutant p53 (p53L194F), to ascertain its biological role in this context, we knock-out p53 in RP2s, generating RP2-p53KO cells, and found that upon complete p53 depletion, p21 levels remained readily detectable (Supplementary Fig. 4B). Furthermore, 2D growth assays showed that the loss of p53 did not impair the proliferation of RP2-p53KO cells in comparison to RP2-Scr (Supplementary Fig. 4C), indicating that the p53 L194F mutation does not exert growth-promoting effects and that p21 expression in BYL719-resistant cells is driven by p53-independent mechanisms.
Next, to assess whether p21 was able to regulate the proliferative capacity of RPs, we utilized our computational models and simulated the effect of varying p21 levels on key markers of cell cycle progression and proliferation. Using the parental PI3K model, we predicted that graded increases in p21 levels would upregulate cyclin D1, inhibit Rb, and increase phospho-S6 (Fig. 4a). Moreover, the resistant PI3K model estimated that diminishing p21 levels in RPs would reduce cyclin D1 and phospho-S6 levels, and reactivate Rb, indicating the presence of a crosstalk between these molecules (Fig. 4b). Interestingly, others have previously shown that p21 can positively regulate formation of the cyclin D1-CDK4/CDK6 complex19.
To confirm these predictions and validate a role for p21 in promoting survival of RPs, we targeted CDKN1A (encoding p21) with two independent guide RNAs, and generated RP-p21 knock-down (KD) T47D lines. We found that reduced p21 levels decreased cyclin D1 levels (Fig. 4c and Supplementary Fig. 5A) and significantly impaired the growth capacity of all RPs (Fig. 4d and Supplementary Fig. 5B). Our data also showed that p21KD suppressed phosphorylation of Rb and S6 (Fig. 4c and Supplementary Fig. 5A) and hence abated critical pro-survival signals. Moreover, considering that the functional output of p21 can also be influenced by its localization20, we next quantified the cellular distribution of p21 in the T47D cell series by immunofluorescence (IF). In cells maintained in growing conditions, we observed a nearly equal distribution of p21 between the nucleus and cytoplasm. However, upon BYL719 treatment, there was a marked increase in p21 nuclear localization across all cell types (Supplementary Fig. 5C). Notably, p21 nuclear distribution was significantly more pronounced in RPs than in T47D cells (Supplementary Fig. 5C). This suggests that not only resistant cells exhibit higher levels of p21, but they also display a more pronounced nuclear accumulation of p21 compared to their parental counterparts.
Finally, we investigated the status of p21 in breast cancer patients using public datasets (METABRIC and TCGA). We confirmed that ~4% of breast cancer patients displayed amplification/ increased expression of CDKN1A compared to average levels across all samples (Supplementary Fig. 5D)20. We then focused on breast cancer samples with PIK3CA mutations and observed that PIK3CA-mutant patients with high CDKN1A expression were associated with poorer overall patients survival compared to patients with mutant PI3K but lower CDKN1A levels (Fig. 4e). Notably, this correlation was not found in PIK3CA wildtype patients (Fig. 4f). We also studied the association between cyclin D1 and PIK3CA mutations given the established oncogenic role of cyclin D1 in breast cancer, and its deregulation in our experimental system. Surprisingly, high CCND1 levels did not predict outcomes in breast cancer patients, irrespective of the PIK3CA status (Supplementary Fig. 5E, F). Thus, these findings suggest a unique cooperation between PI3K and p21 in breast cancer malignancy.
To further corroborate these findings, we next generated T47D cells resistant to the pan-PI3K inhibitor BKM-120. We found that also in response to this alterative targeted therapy, the resulting resistant pools displayed increased p21 levels compared to control cells (Supplementary Fig. 5G). This indicates that selection of high-p21 levels plays a protective, pro-survival role in the face of diverse PI3K-based therapeutic challenges.
Evasion of cellular senescence overcomes the anti-proliferative effect of BYL719
The cytostatic effect induced by BYL719 prompted us to test whether this cellular state was associated with therapy-induced senescence (TIS). To test this, we scored percentages of cells positive to the senescent marker β-galactosidase (β-gal) in parental, RPs and RPs-p21KD T47D cells upon BYL719. We found that parental cells showed low levels of senescence under standard growing conditions (~7%) (Fig. 5a), and that addition of BYL719 for 48 h significantly increased the β-gal positivity (~55%) (Fig. 5a). RPs also showed low senescence in standard conditions (~3%), but the addition of BYL719 only mildly increased the percentage of β-gal cells (~13%), which remained significantly lower than that observed in parental cells (Fig. 5a). Next, we quantified the senescence in RP-p21KD pools and found that p21 knock-down in RPs restored percentages of β-gal positivity to similar levels observed in parental cells (~40%) (Fig. 5b). These data collectively indicate that BYL719 treatments induce a potent senescence response in parental T47D cells and that selection of high-p21 contributes to bypassing this cytostatic condition. We also tested whether alterations in p16, another critical regulator of cellular senescence occurred in these cells and found that p16 levels remained unchanged in parental and RPs even when these were treated with BYL719 (Supplementary Fig. 6A). This demonstrates that p21 plays a unique role in overcoming the BYL719-induced senescence response.
We next asked whether PDK1 inhibition, like PI3Kα inhibition, causes TIS. We found that treatment with the PDK1 inhibitor GSK2334470 resulted in a threefold increase in senescence in T47D parental cells compared to DMSO-treated cells (Supplementary Fig. 6B). However, in RPs, GSK2334470 only caused minimal β-gal staining (Supplementary Fig. 6B). This indicates that similar to PI3K inhibition, PDK1 inhibition triggers senescence in sensitive cells, albeit to a lesser extent than that observed with BYL719. Moreover, in 2D growth assays (Fig. 2i) we observed that BYL719-RPs proliferated more rapidly than parental T47D cells even when treated with GSK2334470, indicating that acquisition of resistance to PI3K inhibition also confers resistance to single PDK1 inhibition.
Genomic instability is a vulnerability of BYL719-resistant breast cancer cells
Senescence defines a quiescent cell state that can be induced by DNA damage. To explore whether the senescence observed in BYL719-treated T47D cells was associated with damage to DNA, we immuno-stained the T47D cell series with the DNA damage marker γ-H2AX and 53BP1. We found that 48 h of BYL719 treatment doubled the γ-H2AX positivity in parental cells, reaching levels significantly higher than those observed in RPs (Fig. 5c). Similarly, T47D cells showed diffuse 53BP1 nuclear staining in DMSO which became localized in intense nuclear foci upon BYL719 treatment; similar to γ-H2AX, the intensity of 53BP1 nuclear foci was higher in parental cells than RPs (Fig. 5d).
Importantly, p21KD rescued the γ-H2AX intensity in RPs, i.e., RP-p21KD cells, compared to control samples (Fig. 5e). This led us to conclude that prolonged PI3K inhibition causes DNA damage-induced senescence and that selection of high-p21 levels contributes to repair the damaged DNA and promotes exit from this arrested cell state.
Given the increased DNA damage caused by BYL719 in T47D cells, we next wondered whether targeting DNA damage response pathways could provide a valuable approach to complement PI3Kα inhibitors in the treatment of resistant cells. To this end, we focused on essential regulators of the G2-to-M cell cycle checkpoints whose blockade induces death of p53-mutant cells, such as the T47D cells21. First, we found that RPs showed higher phosphorylation levels of CHK1-Ser345, ATR-S428 and BRCA-S1524, confirming that these cells have heightened activation of DNA damage repair and replication checkpoints (Figs. 5f and 6a). Second, we tested the cell viability of T47D cells upon increasing concentrations of the CHK1 inhibitor MK-8776 (Fig. 6b). We found that 3 days of MK-8776 treatment mildly but significantly limited survival of parental cells and RPs, and caused a small percentage of cell death (Fig. 6c). However, in combination with BYL719, CHK1 inhibition effectively constrained cell growth in parental cells (Fig. 6b) and also rescued the sensitivity of RPs to BYL719 (Fig. 6d). Importantly, this effect was associated with increased DNA damage (Fig. 6e), which not only partially rescued the senescence response in RPs (Fig. 6f), but significantly enhanced their cell death compared to single-drug treatments (Fig. 6g).
These data indicate that blocking CHK1 in combination with BYL79 provides an effective therapeutic approach to specifically target and kill BYL719 resistant cells (Fig. 6h).
Extending the applicability of experimental and in silico models
To broaden the scope of our findings, we tested the response of the osteosarcoma Saos2 cell line to BYL719, as these cells demonstrated resistance to anti-cancer treatments following induced p21 expression22. To this end, we chronically exposed three independent plates of Saos2 cells to increasing concentrations of BYL719 (starting at IC50: 2 μM), or DMSO (similar v/v) as control. We generated 3 BYL719-resistant cell lines (BY-1, BY-2, and BY-3) and confirmed that they proliferated more rapidly than control cells in the presence of BYL719 (Fig. 7a). Importantly, we detected elevated levels of p21 and CHK1 phosphorylation in BYL719-resistant cells compared to control samples (Fig. 7b). Consistently, a combination treatment of BYL719 and the CHK1 inhibitor MK-8776 effectively suppressed the growth of both cell types. These data further support a role for high-p21 in drug resistance, and highlight the efficacy of co-targeting PI3K and CHK1 in therapy-resistant cells, especially those with mutations in PI3K and p53 (Fig. 7c).
We next sought to evolve the in silico PI3K network model to generate a phenomenological model that integrates major cell cycle phases (encompassing G1, S, G2/M phases) and key phenotypic outputs (i.e., DNA Repair, and Apoptosis). This phenotypic model also incorporates DNA Damage (DD) and CHK1 activity as explicit model components to trigger biological outcomes: DNA repair and cell viability, or apoptosis (Fig. 7d). Using a similar simulation approach as with the original model, we determined the impact of co-inhibiting each node of the evolved phenotypic model (n = 25, including CHK1) in conjunction with PI3Kα on cell viability. A detailed description of the construction of the new model along with model assumptions is provided in the 'Construction of the phenotypic model‘ section of the Methods; while detailed rate equations and kinetic parameters are provided as Supplementary Table S4 and Supplementary Dataset 3.
Model simulations revealed that co-inhibition of PI3Kα and CHK1 exhibited a marked synergistic effect on suppressing cell viability, ranked as the second most potent combination among all the evaluated pairs (Fig. 7e). Co-inhibition of PDK1 and PI3K remained the most synergistic combination (see Fig. 2a–f), indicating the essential role of full PI3K pathway inhibition for cancer suppression. Notably, the order of synergistic drug pairings obtained from the phenotypic model closely aligned with the predictions from the original PI3K model, reinforcing the experimental synergy observed with CHK1 and PI3K inhibitors.
Discussion
We have integrated computational and experimental approaches to tackle an important question in breast cancer treatment: resistance to oncogene-based targeted therapies. We have studied molecular responses of a PIK3CA-mutant, ER+ breast cancer cell line to short-term and chronic exposure to BYL719, and defined signaling adaptations within the PI3K network that cause drug resistance. Our model predictions show that PDK1 is the most effective target enhancing the antitumor activity of BYL719 in sensitive and resistant T47D breast cancer cells. Modeling showed that PDK1 plus PI3Kα inhibition display the highest synergistic drug-score, superior also to compounds targeting mTORC1 or cyclin D1 (Fig. 2a–f), which translated into stable inhibition of markers of proliferation and growth suppression of resistant cells (Fig. 2h, i). Thus, consistent with studies emphasizing a role for PDK1 in promoting breast cancer malignancy23, our predictions indicate that PDK1 is also a prominent target for the treatment of resistant disease in ER+ breast cancers with PIK3CA mutations. Notably, the in vivo efficacy of this drug combination was previously reported in pre-clinical model of breast cancers10. Our modeling also supports the notion whereby in a context in which AKT is still inhibited (Fig. 1g) compensatory PDK1 activation in response to BYL719 rescues a pro-growth signal by engaging with the SGK1/3 kinases10,24. Consistently, RPs show higher phosphorylation of the SGK1-target NDRG1 than parental T47D cells (Supplementary Fig. 2A). Thus, by building and training new in silico models, we have generated new tools that accurately predict effective combinatorial therapies directed at key components of the PI3K pathway. These tools can guide the prioritization of combinatorial treatments when monotherapies fail.
Several oncogene based-targeted therapies have been approved for breast cancer, however, lack of predictive biomarkers of response remains a clinical hurdle5. Rapalogs and inhibitors of CDK4/CDK6 ribociclib and palbociclib can improve response of ER+/HER2− breast cancer to hormone therapies, but how to best identify which patient benefits from one or the other therapy is unknown25. Our in silico approach offers the ability to capture context-specific and dynamics of cellular responses to clinically relevant drugs, and provides a new means to analyze personalized treatments for PIK3CA-mutant patients. In future, these models can be integrated with additional datasets into unified quantitative frameworks to rationally design and prioritize therapeutic strategies for different types of breast cancers, or malignancies, with PI3K alterations.
Beyond the PI3K network, we have also shown that T47D cells become resistant to BYL719 thanks to the pro-survival effect induced by the selection of high-p21 levels. Better known as the CDK inhibitor downstream to the tumor suppressor p53, p21 has been shown to regulate several biological processes in response to DNA damage, in a p53-independent manner20. Upregulation of p21 in response to oncogene induced DNA-damage (e.g., PML-RARα) was reported to promote DNA repair and contributed to stem cell maintenance in the hematopoietic and mammary epithelial compartments26,27. By interacting with the proliferating cell nuclear antigen (PCNA), p21 can displace DNA replication enzymes and blocks DNA synthesis in favor of DNA repair28. Consistently, we now show that p21 upregulation also occurs in T47D cells and Saos2 cells upon chronic BYL719 treatments and, by promoting repair of damaged DNA, high-p21 favors bypass of therapy-induced senescence (TIS) (Figs. 5 and 7a–c). Our findings provide multiple new insights into the events that ultimately cause resistance to PI3Kα inhibition. First, we found that the BYL719-induced cytostasis is associated with a senescence response. While TIS has been observed in vitro and in vivo29, including human studies in response to chemotherapies30,31 we add that this also occurs in response to PI3Kα inhibition, and PDK1 inhibition (Fig. 5a and Supplementary Fig. 6B). Second, we find that the BYL719-induced senescence is associated with DNA damage, consistent with reports showing that the pan-PI3K inhibitor BKM120 and BYL719 itself decrease de novo nucleotide synthesis and cause replication stress in breast cancer models32. Third, unlike the common knowledge whereby p21 promotes senescence20, we find that selection of high-p21 favors evasion of this cellular defense mechanism by promoting repair of damaged DNA. Evasion of cellular senescence has been associated with selection of tumor cells with stem-like properties33 and importantly, that p21 upregulation promoted senescence bypass was previously reported in response to chemotherapeutic agents22. In Li Fraumeni-derived fibroblasts and Saos2 osteosarcoma cells with p53 loss, forced p21 expression caused an initial senescence response but also favored selection of escaped cells with even higher p21 levels, aggressive phenotypes, and resistant to doxorubicin and cisplatin22. More recently, high-p21 levels were shown to promote tumor growth and resistance to HER2-targeted therapies in HER2 and PIK3CA mutant breast cancers34. Thus, we conclude that high-p21 levels can be used as a biomarker to identify tumor cells with potential acquired resistance to systemic and targeted therapies inducing DNA damage.
Further, the dependency between high-p21 and repair of DNA damage is underscored by the efficacy with which CHK1 inhibition and BYL719 increase death rates of RPs (Fig. 6f), but show low toxicity on quiescent, parental T47D cells (Fig. 6c). CHK1 is a target of the ATM/ATR kinases and is activated in response to DNA damage and replication stress35, and controls replication initiation forks36. CHK1 loss can lead to mitotic catastrophe and death in cells with Tp53 alterations which have lost control of the G1/S checkpoint, and rely on G2/M checkpoint regulators such as CHK1 to safeguard genome stability21. By inhibiting CHK1 activity in cells that depend on DNA repair for survival, such as the BYL719-resistant cells, we propose a new synthetic lethal approach based on PI3Kα inhibition. Importantly, the synergism between CHK1 inhibition and inhibition of PI3K pathway components has been observed also in triple-negative breast cancer (TNBC) cell lines with mutations in PI3K, PTEN, plus p5337, and extends to high-grade serous ovarian carcinoma38. Thus, in a mutant p53 background, high-p21 level sensitizes cells to compounds that target DNA synthesis and DNA repair, and defines a vulnerability of cells treated with DNA damaging agents, including PI3K inhibitors.
Finally, we assessed whether PDK1 inhibition affected p21 levels in parental and RPs and noticed that when combined with BYL719, GSK2334470 decreased p21 levels (Fig. 2h). Interestingly, p21 protein stability is controlled by the mTORC1 substrate 4EBP1, and active mTORC1 leads to higher p21 protein levels39. Therefore, by repressing mTORC1 activation, PDK1 inhibition also affects p21 protein stability and defines a strategy to limit p21 upregulation.
Collectively, in this study we have generated new computational tools and identified critical genetic determinants causing resistance to PI3K-based therapies and propose new combination treatments for PIK3CA-mutant resistant breast cancers.
Methods
Computational modeling
Mathematical models were formulated using ODEs based on synthesis of model components and network interactions. Detailed accounts of model reactions, reaction rates and equations are included in Supplemenatary Tables S1 and 2. Model construction and simulation were implemented in MATLAB in conjunction with the IQM toolbox (https://iqmtools.intiquan.com/). The parental PI3K model was fitted to experimental data and parameter estimation, and was implemented using genetic algorithms as part of the Global Optimization Toolbox in MATLAB. Values of all best-fitted parameter sets are provided in Supplementary Dataset 1.
The resistant PI3K model was derived from the parental model by adjusting initial conditions of model species between parental and RPs, guided by experimental measurement. Details on model generation, scope and assumptions, as well as model fitting are provided in the Supplemental Information.
Mathematical model description and assumptions
To systematically and quantitatively interrogate the dynamic cellular response to drug treatments and the adapted behaviors of the PI3K signaling network, we constructed a dynamic mathematical model that integrates canonical components of the PI3K pathway and major reported signaling axes implicated in the acquired resistance to PI3K inhibition.
Upstream receptor tyrosine kinases (RTKs)
The PI3K pathway sits downstream multiple RTKs including the IGF-1R/IR and ErbB families of tyrosine kinase receptors40,41, which have been shown to confer resistance to PI3Kα inhibition42,43,44. Thus, IGF-1R/IR and ErbBs were chosen as single model species, each representing their respective RTKs family. In addition, ErbB2 (HER2) and ErbB3 (HER3) are the most abundantly expressed members of their RTKs family in T47D cells45, and act as preferred binding partners among the ErbB family receptors, thus defining prototypical molecules in our model system46.
Our model incorporates the p110α and β isoforms of PI3K and their key downstream effector signaling axes, such as AKT/mTOR/S6K1/S6, SGK3/NDRG1, SGK1/FOXO3, P-Rex1/Rac1 and c-Myc (Fig. 1a). Their inclusion is based on studies showing that p110β and SGKs confer resistance to isoform selective or pan-PI3K inhibitors42,47,48. Our model also includes the Ras/Raf/MEK/ERK MAPK signaling pathway, a major crosstalk pathway that displays reciprocal interplay with the PI3K signaling and frequently confers resistance to inhibitors targeting PI3K/AKT signaling41,49. Both IGF-1R/IR and ErbB can promote activation of the p110α/β/PIP3/PDK1-AGC protein kinase family (AKT, SGK1, and SGK3) pathways; and ErbB directly activates the Ras-Raf-MEK-ERK pathway, as shown in Fig. 1a.
Cell cycle machinery
An important feature of our mechanistic model is the incorporation of the critical cell cycle machinery (CDKs/Rb/Cyclin D/E/E2F and p21), downstream PI3K/AKT/mTOR and the Ras/MAPK pathway. We assumed that mTORC1 controls the translation of c-Myc and cyclin D1 mRNA by activating eukaryotic translation initiation factor 4E (eIF-4E)50,51. The transcriptional repressor activity of Rb can be antagonized by sequential phosphorylation events, initiated by cyclin D1-CDK4/6 in early G1 phase, followed by cyclin E-CDK2 in late phase52. Hyper-phosphorylated Rb loses its association with chromatin to release its suppressive role on E2Fs in the nucleus53. E2Fs induces expression of cyclin E independently and also in collaboration with Myc54, as shown in Fig. 1a. The model also includes the positive auto-regulation of E2F54. Expression of p21 was assumed to be regulated by ERK55. Furthermore, AKT phosphorylates p21 and enhances its protein stability, which promotes cell survival56.
Major feedback loops and crosstalk mechanisms
Signaling dynamics and drug response behaviors are strongly determined by the presence of positive and negative feedback interactions within signaling networks41,57. Thus, our model aimed to capture these events through a careful synthesis of the literature. Below we discuss the salient mechanisms included in the model.
Rb-mediated feedback to mTORC2/AKT
We assumed that hyper-phosphorylated Rb directly suppresses the kinase activity of mTORC2 toward its substrate AKT. This was because phosphorylated Rb binds Sin1, an integral component of mTORC2, thereby blocking AKT access to mTORC2, and ultimately leading to attenuated AKT activation58. This constitutes a negative feedback loop between Rb and mTORC2/AKT.
Cyclin D1-CDK4/6 mediated feedback loop
Another feedback loop emanating from the cell cycle module to an upstream pathway is governed by cyclin D1-CDK4/6 complex, which phosphorylates and inhibits TSC2 at Thr-146259. This effectively generates a positive feedback between Cyclin D1-CDK4/6 and mTORC1, as shown in Fig. 1a.
S6K-mediated negative feedback loop
There are a number of known negative feedback loops originating from mTORC1 that ultimately limit PI3K/AKT activation, including one mediated by S6K and one by Grb10, both acting through IRS1/22. Although these feedback mechanisms are biochemically distinct, functionally they act in a similar manner, that is to shut down PI3K/AKT activation when it is exceedingly high. Thus, to keep the model simple yet biologically relevant, we only included the S6K-mediated feedback loop60,61,62.
GAB-mediated feedback loop
A major role of PI3K is to catalyze PIP2 phosphorylation to PIP2. In the model, we assumed that PIP3 in turn can recruit the adapter proteins GAB1/2, which enhances PI3Kα and β activation through association with the p85 subunit of PI3K63,64,65. Effectively, these interactions create positive feedback loops between PI3K and GAB1/2.
P-Rex1-mediated feedback loop
P-Rex1 is a guanine nucleotide exchange factor (RacGEF) of Rac1, which promotes the activity of Rac1. Interestingly, P-Rex1 is activated by PIP366,67,68. Moreover, p110β is a direct Rac1 target, and Rac1 activates p110β69. Thus, these interactions form a positive feedback loop between P-Rex1 and p110β via Rac1 and PIP3, as shown in Fig. 1a. In addition, P-Rex1 catalyzes the activation of Rac1, which sequentially stimulates the kinase activity of PAK170. PAK1 enhances ERK signaling by phosphorylation of Raf-1 (S338) and MEK1 (S298)71,72,73. For simplicity, we assumed that Rac1 directly phosphorylates MEK.
ERK-mediated feedback loops
Multiple negative feedback mechanisms are induced by ERK towards upstream signaling components, including Raf, Ras and RTKs74. In our model, we included two ERK-mediated negative feedback loops on Ras and ErbB as representatives of a short- and long-feedback loop (Fig. 1a) in a nested feedback structure. We have previously demonstrated that individual feedback loops within coupled structures like this possess distinct dynamics-modulating function74, thus supporting the explicit modeling of two ERK-mediated loops.
FOXO3-mediated feedback loop
Both AKT and SGK1 phosphorylates FOXO3 at residues T32, S253 and S315, which promotes FOXO3 binding to 14-3-3 proteins and decreases its interaction with transcription coactivators CBP/p30075,76; note that SGK1 has a marked preference for Ser-315, whereas AKT favors Ser-25376. FOXO3 binds to S1/S4 on the ESR1 promoter and induces ERα expression77.
ER-mediated feedback loops
The estrogen receptor (ER) plays a key role in the progression of breast cancer, particularly the luminal subtypes that encompass the T47D cell line. Once bound by estrogens, ER dimerizes and translocates to the nucleus where it interacts with transcriptional proteins78. In the model, we assumed that ERα induces the expression of c-Myc79 and promote the expression of SGK380,81. ERα signaling is also regulated by other network components, including FOXO3 and ERK. FOXO3 is known to bind to the ERα promoter and enhance ERα signaling77; and ERK1/2 phosphorylates ERα at a number of serine sites which increases its activity82. These interactions are captured in our model, as displayed in Fig. 1a.
NDRG1-mediated feedback loop
In the model, we assumed that ErbB is negatively regulated by NDRG1 since NDRG1 enhances the interaction of ErbB with the ubiquitin ligase NEDD483,84. Furthermore, NDRG1 is phosphorylated by SGK1/3 at T346/T356/T366, priming it for further phosphorylation by GSK-3β at S342/S353/S46285,86. Phosphorylation by GSK-3β is a common priming event for ubiquitination by the E3 ligase SCF complex Fbw786. Thus, Fbw7 targets NDRG1 for degradation by the 26S proteasome86.
Other crosstalk mechanisms
There are multiple reciprocal crosstalk mechanisms between the PI3K/AKT and Ras/ERK pathways. In the model, we assumed that Ras directly activate PI3Kα through interacting via an amino-terminal Ras-binding domain (RBD)69. In the opposite direction, AKT phosphorylates and inhibits Raf, which leads to inhibition of the Raf/MEK/ERK cascade87,88, providing another crosstalk point between the two pathways. In addition, ERK phosphorylates GAB1 at six serine/threonine residues (T312, S381, S454, T476, S581, S597)89, which inhibit GAB1/PI3K association and thus suppresses the activity of PI3K90. ERK can also phosphorylate GAB2 and negatively regulates p85 recruitment91. Thus, in the model we assumed that ERK inhibits GAB, providing another crosstalk point between the two pathways.
Model implementation
The new PI3K-centered model was formulated using ordinary differential equations (ODEs) following the interaction map depicted in Fig. 1a. The rate equations and full set of ODEs are given in Supplementary Tables 1 and 2. The model was implemented and numerically solved using MATLAB in conjunction with the IQM Tools (https://iqmtools.intiquan.com/) and the SUNDIALS suite (SUite of Nonlinear and DIfferential/ALgebraic equation Solvers, https://computing.llnl.gov/projects/sundials).
This combination of tools provides a scalable and powerful approach to construct and simulate ODE models of medium to large size, such as our model. Specifically: (1) an ODE function file containing definition of all model reactions, reaction rates and rate equations is created in IQM Tools based on the IQM syntax; (2) the ODE function file is transformed into C source code by IQM; (3) MATLAB then compiles and links the C code and SUNDIALS libraries into a binary MEX file; (4) and finally the MEX file is used for numerical solving by SUNDIALS’s ODE solver package CVODE. The main reason we employed SUNDIALS is because CVODE is significantly faster (~10 times) than conventional MATLAB solvers such as ODE15s in solving stiff and non-stiff ODE systems. Note that the speed may depend on a complexity and stiffness of the ODE systems. Essentially, the IQM toolbox provides an efficient MATLAB interface to SUNDIALS’s CVODE package.
Model calibration and generation of “parental PI3K model”
Kinetic parameters in dynamic models are not determined experimentally and require calibration, or fitting, through experimental data to estimate unknown parameters. The potential discrepancy between simulated model output and experimental data can be minimized to find the best parameter values92,93. Model calibration is a critical step that provides a specific biological context to an otherwise ‘generic’ model. In this study, parameter estimation was performed by identifying the parameter set p in order to minimize the following ‘objective function’ that quantifies the mismatch between experimental measurements and corresponding simulated outputs94:
where M is the number of the experimental datasets used for fitting; N is the number of time points within each dataset; yj (ti,p) represents the numerically solved value of the model state variable yj evaluated at time ti and parameter set p; while yDj,i is the mean value of the corresponding data point at ti with the associated variance of measured data σj,i. Note that when averaged or single valued data are used, σj,i is set to be 195.
Model calibration for T47D parental cells
We first generated a ‘parental model’ by performing model calibration using datasets obtained exclusively from the parental T47D breast cancer cell line. These include time-course and dose-response data of phosphorylated AKT and ERK, and expression of Cyclin D1 and p21 in response to stimulation by IGF-1, insulin and HRG, which were quantified and presented in Fig. 1b. ERK1/2 and AKT phosphorylation data by IGF-1 were downloaded from HMS LINCS Center (https://www.cancerbrowser.org/). ERK1/2 and AKT phosphorylation data and total level of cyclin D1, Myc and p21 by HRG were sourced from Neve et al., T47D cells15. Dose-response data of pAKT and pERK levels upon HRG stimulation were obtained from Neve et al., T47D cells15. Dose-response of pAKT, pERK and pS6 levels in T47D cells upon insulin stimulation were obtained from in-house experiments.
Genetic algorithm specification
We employed a genetic algorithm (GA) to optimize the objective function J due to its ability to avoid being trapped in local minima, use probabilistic selection rules, and based on our experience, work well for ODE models with a large number of parameters96,97,98. This was implemented using the Global Optimization Toolbox and the function ga in MATLAB. Selection rules select the individual solutions with the best fitness values (i.e., elite solutions) from the current population. The elite count was set to 5% of the population size. Crossover rules combine two parents to generate offspring for the next generation. The crossover faction was set at 0.8. Mutation rules apply random changes to individual parents to generate the population of the next generation. For the mutation rule, we generated a random number from a Gaussian distribution with mean 0 and standard deviation σk, which was applied to the individuals of the current generation. The standard deviation function (σk) is given by the recursive formula as follows:
where k is the kth generation, G is the number of generations, and σ0 = 1.
Calibration implementation
Due to the size of our model, model calibration was carried out on a multi-processor virtual server consisting of 32 Intel Xeon 2.10 GHz processors running in parallel. To derive at the best fitted parameter set, we performed repeated GA runs with population size of 2000 and the generation number set to 100. During these runs, we also changed the mutation rate, crossover rate and even the population size in order to escape from being trapped in local minima99. After multiple repetitions of the GA process where the best fitted set obtained from a previous repeat was used as the starting point of the next repeat, we arrived at a best fitted set as the objective function was not further reduced, and the fitted parameter values no longer change.
Ensemble simulation to mitigate issues with model unidentifiability
Dynamic models in systems biology, particularly those of large size, face challenges of poor identifiability. This is primarily due to a lack of informative experimental data, and the existence of ‘local minima’ in the objective function landscape100. Thus, generally there is a trade-off between model identifiability and level of biological details. In this regard, our PI3K model suffers from unidentifiability because of its detailed scope and interactions, which were a deliberate design decision as we aimed to capture mechanistic feedbacks and crosstalk between multiple related pathways, and to facilitate a comprehensive prediction of drug response and drug combinations. To cope with this issue, we employed a two-pronged approach. First, we avoided the reliance (and possible biases) on a single best-fitted parameter set by repeating the GA-based procedure described above hundreds of time, each time with a different initial guess (generated from a log-uniform distribution in a range between −3 and 3), to obtain a final total of 77 independent best-fitted parameter sets that fitted the training data equally well (see Supplementary Fig. 1B and Supplementary Information). Critically, rather than using any single sets, we utilized all the obtained sets collectively for subsequent simulation and analysis, considering explicitly the mean and variance of simulated behaviors. This ‘ensemble’ strategy thus allows us to generate high-confidence predictions without strictly imposing identifiability on our model. Second, to gauge the calibrated model’s predictive power before making entirely new predictions, we further validated it with independent datasets that were not used during calibration (for example, see Supplementary Fig. 1A–D and relevant discussion in the main text). Together, our approach helps maximize the predictive capability of our parental model.
Generation of “resistant PI3K model”
To generate a model describing the state of T47D cells resistant to BYL719 (called the resistant PI3K model) we comparatively profiled the basal (i.e., under standard growing condition) expression and/or phosphorylation levels of key network components between resistant and parental T47D cells. We next utilized this data to modify the basal signaling levels of the parental model and produced the resistant PI3K model. For example, our data showed that the expression levels of p21 and Cyclin D1 were about 7 and 3 folds higher in resistant cells than parental T47D cells, respectively; while the levels of AKT and ERK are relatively similar between the two cell types (Supplementary Fig 2C, D). Thus, in the resistant model, the initial concentrations of p21 and Cyclin D1 were adjusted accordingly to reflect the differential values in expression. This model customization strategy has been previously employed by us95,101 and others102, and proved to be a simple yet efficient strategy to specify models with the same network wiring to different biological contexts.
Construction of the phenotypic model
Our data shows that BYL719 treatment causes DNA damage in T47D cells (Figs. 5 and 7d). Accumulation of DNA damage can prompt cells to initiate apoptosis and prevent proliferation of damaged cells. A crucial early step in this process involves the recruitment of the Mre11/Rad50/NBS1 (MRN) complex to double-stranded DNA break sites103,104,105. This action primes ATM activation, culminating in its auto-phosphorylation. Concurrently, ATR becomes active and similarly undergoes auto-phosphorylation. Once activated, both ATM and ATR phosphorylate a number of downstream targets, notably c-Abl (a non-receptor tyrosine kinase that phosphorylates the BH3-only protein Bim, countering the anti-apoptotic process) and specific caspases (namely caspase-8, -9, and -3)106,107,108.
For model simplicity, we assumed that DNA damage directly promoted apoptosis. The model also incorporates DNA damage-driven CHK1 activation, given that both ATM and ATR phosphorylate CHK1109. Once activated, CHK1 orchestrates the phosphorylation of diverse targets, including CDC25A, B and C, as well as p53110. This phosphorylation cascade inhibits CDC25A, B and C, blocking the transition to the G2/Mitosis phases. Concurrently, CHK1 also promotes DNA repair (R) by regulating the expression of DNA repair genes through activation of the transcription factor GADD45111,112. Importantly, Cyclin D1 and cyclin E, outputs from the mechanistic PI3K network model, drive the transition from G1 to S phase and act as inputs into the phenomenological model, thereby linking these two models to make up the new phonotypic models.
As with the original models, the phenotypic model was formulated using ordinary differential equations (ODEs) based on established kinetic laws95,101 (Supplementary Table 4). The model was then used to assess the impact of co-inhibiting PI3K with each of the 25 model nodes, including CHK1 as co-target, on cell viability. Cell viability was defined as the number of cells in DNA repair phase (R) or in G2/M phase (M), the latter emerging from successful DNA repair (Fig. 7d).
Establishment of cell lines resistant to targeted therapies
The T47D human breast cancer cell line was purchased from the ATCC and cultured in RPMI1640 media supplemented with 10% fetal calf serum, 0.2 Units/ml of insulin, and 1% penicillin/streptomycin, as recommended. T47D cells were split in 1:3 to 1:4 twice a week. Cells with passage number lower than 20 were used in all experiments. To establish BYL719-resistant cell pools, T47D cells (200,000 per well in a 6-well plate) were exposed to increasing concentrations of BYL719 (Selleckchem, #S2814), starting with 1 μM and up to 30 μM, over 2 months. T47D resistant pool 1, 2 and 3 (herein RP1, RP2 and RP3) were generated and maintained in 1 μM BYL719, pulsed every 2 days. Similar procedures were used for the generation of T47D cells resistant to BKM-120 (Supplementary Fig. 5G).
For Saos2 cells, three independent plates of cells were chronically exposed to increasing concentrations of BYL719 (starting at 2 μM), or DMSO (similar v/v) for comparison. DMSO-treated cells reached confluency every 4–5 days, BYL719-treated cells remained quiescent for several weeks. However, after 6 weeks, BYL719-treated cells started to proliferate and to grow under selection.
CDKN1A and Tp53 knock-down via CRISPR/Cas9
The Alt-R CRISPR-Cas9 System kit (Integrated DNA Technologies) was used to knock-down CDKN1A (p21) and TP53 in T47D cells according to the “Cationic lipid delivery of CRISPR ribonucleoprotein complex into mammalian cells” user guide Version 3. Briefly, a Cas9:crRNA:tracrRNA ribonucleoprotein (RNP) complex was generated by mixing equimolar concentrations of crRNA and tracrRNA stocks in nuclease-free duplex buffer, followed by the addition of the Cas9 enzyme and Cas9 PLUS reagent, mixed in Opti-MEM medium. Two independent crRNAs targeting CDKN1A (i.e., AB and AD) and one targeting Tp53 (i.e., AA) were used in this study. Transfection was performed by mixing 400,000 T47D RP cells with the RNP complex and lipofectamine 3000 in a 12-well plate. Cells were left undisturbed in a tissue culture incubator (37 °C, 5% CO2) for 48 h, after which complete RMPI medium with 10% FBS was used. CDKN1A knock-down was assessed by Western blotting using the indicated p21 and p53 antibody.
Cell growth assays
T47D cells were plated in 24-well plates (25,000 cells/well) in full growth medium and left to attach overnight. The day after, one of the plates was washed in 1X PBS and fixed in 10% formalin at room temperature (RT) for 15 min, then washed with 1X PBS twice and stored at 4 °C until the end of the experiment (Day 0 plate). Remaining plates were treated as indicated in figures, and fixed on day 2, 4 and 6. At the end of the assay, cells were stained with crystal violet solution (0.1% (w/v) crystal violet in 20% methanol/dH2O at RT for 30 min. Each well was washed in 1X PBS three times and air dried overnight. Cell-bounded crystal violet was extracted in 10% (v/v) acetic acid solution for 30 min. Solutions were transferred to a 96-well plate and their absorbance measured at 590 nm using a PHERAstar FSX plate reader.
Protein lysates and immunoblotting
T47D cells (150,000 cells/well) were plated in 6-well plates and treated as indicated. Standard protocols were used for western blotting analyses. At the end of each experiment, cells were washed in ice-cold PBS, scraped in RIPA lysis buffer (20 mM Tris-HCl pH7.8, 150 mM NaCl, 1% (v/v) NP-40, 0.05% (w/v) Sodium Deoxycholate, 0.4% (w/v) SDS, supplemented with 1X complete protease inhibitor (Roche) and 1X PhosSTOP (Roche)). Lysates were sonicated and cleared by centrifugation. Standard Laemmli-Buffer with 10% final concentration of β-mercaptoethanol was added and samples boiled for 5 min, resolved in NuPAGE Bis-Tris 4–12% protein gels (Life Technologies), and transferred onto nitrocellulose membranes. Membranes were blotted for 1 h in 5% (w/v) skimmed milk/ TBS-T (0.1% Tween 20 in Tris-buffered saline) and probed with the indicated primary antibodies in 5% (w/v) bovine serum albumin (BSA)/TBS-T overnight at 4 °C. After 3 washes in TBS-T buffer, membranes were probed with Amersham ECL horseradish peroxidase (HRP)-secondary antibodies (GE Healthcare) for 1 h at RT, followed by 3 washes in TBS-T buffer. Signal detection was performed by incubating membranes with Pierce ECL Western Blotting substrate followed by x-ray film development. All blots were derived from the same experiments and were processed in parallel. Uncropped scans of the most important blots are provided as Supplementary Figs. 7 and 8 in the Supplementary Information.
3D cell growth assay
Poly-2-hydroxethyl methacrylate (HEMA) solution (3% w/v) was prepared by dissolving poly-HEMA (Sigma-Aldrich, P3932) in 95% ethanol at 37 °C overnight. Wells of 24-well plates were coated with 400 μl poly-HEMA solution overnight. T47D cells (30,000/well) were plated and treated as indicated for 4 days. At the end of the treatment, cell aggregates were collected by centrifugation and dissociated with trypsin for cell counting.
Proteomics
Culture of T47D cells and cell lysis
T47D cells, parental and resistant pools, were plated in 15 cm dishes, let to seed for 48 h and then treated with 1 μM BYL719 for 24 h before harvest. Cells were scraped off in growth medium and spun at 250 × g for 10 min at RT. Cells were washed with 1X PBS at 320 × g for 7 min, cell pellets were lysed in RIPA buffer containing protease inhibitor (Roche) and 1X PhosSTOP (Roche, in HPLC-grade water) on ice for 5 min, and then sonicated and cleared at 4 °C by centrifugation.
Protein precipitation and digestion
Cell lysates were precipitated in 5X volume of ice-cold acetone at −20 °C overnight. Protein precipitates were spun at 17,000 × g for 10 min at 4 °C and washed once in ice-cold acetone. Proteins were re-solubilised in 8 M urea buffer containing 10 mM tris(2-carboxyethyl) phosphine (TCEP) assisted by sonication. Protein concentration was quantified and samples normalized to the same volume. Samples were then alkylated in 55 mM iodoacetamide for 45 min in the dark. Urea in samples was diluted to 1 M with 25 mM triethylammonium bicarbonate (TEAB), pH 8.0 before digestion with Pierce™ Trypsin Protease, MS Grade (Thermo Fisher Scientific, #90059) at 37 °C overnight. Samples were then acidified with formic acid to a final concentration of 1% (v/v).
Samples’ clean-up and phosphopeptide enrichment
Solid-phase extraction (Oasis HLB, Waters, #WAT094226) was used for peptides cleaning. Briefly, cartridges were conditioned with 80% (v/v) acetonitrile/0.1% (v/v) trifluoroacetic acid (TFA) followed by equilibration with 0.1% TFA. Samples were then loaded and allowed to bind to the sorbent in the columns. Columns were then washed twice with 0.1% TFA and peptides eluted in 80% (v/v) acetonitrile/0.1% (v/v) TFA. Samples were freeze-dried overnight. Samples were then resuspended in loading buffer (2 M lactic acid in 50% acetonitrile and 5% TFA) through vortexing and sonication. Titansphere, spherical TiO2 beads (GLSciences, 5020-75000) at a ratio of 6 mg/mg proteins were conditioned by washing in Washing buffer (50% acetonitrile and 5% TFA) followed by Loading buffer. Samples were incubated with 80% of the conditioned TiO2 beads for 60 min with 450 × g shaking and spun down. Supernatants were incubated with remaining TiO2 beads for an extra 30 min. After TiO2 enrichment, beads were packed into a home-made stage tip (a C8 plug in a 200 μl tip). Peptide samples were loaded into the tips and spun through the tips at 1250 × g for 10 min. Tips were then washed with Loading buffer and Washing buffer until all samples were loaded. Phosphopeptides were eluted in 1% (v/v) ammonium hydroxide followed by 30% (v/v) acetonitrile. Samples were freeze-dried overnight.
Data-dependent acquisition (DDA) LC-MS/MS
Samples were analyzed by LC-MS/MS using Orbitrap Lumos mass spectrometer (Thermo Scientific) fitted with nanoflow reversed-phase-HPLC (Ultimate 3000 RSLC, Dionex). The nano-LC system was equipped with an Acclaim Pepmap nano-trap column (Dionex—C18, 100 Å, 75 μm × 2 cm) and an Acclaim Pepmap RSLC analytical column (Dionex—C18, 100 Å, 75 μm × 50 cm). Typically for each LC-MS/MS experiment, 10 μl of the peptide mix was loaded onto the enrichment (trap) column at an isocratic flow of 5 μl/min of 3% CH3CN containing 0.1% formic acid for 8 min before the enrichment column is switched in-line with the analytical column. The eluents used for the LC were 5% DMSO/0.1% v/v formic acid (solvent A) and 100% CH3CN/5% DMSO/0.1% formic acid v/v (solvent B). The gradient used was 3% B to 25% B for 177 min, 20% B to 40% B in 5 min, 40% B to 80% B in 5 min and maintained at 80% B for the final 5 min before equilibration for 10 min at 3% B prior to the next analysis.
The mass spectrometer was operated in positive-ionization mode with spray voltage set at 1.9 kV and source temperature at 275 °C. Lockmass of 401.92272 from DMSO was used. The mass spectrometer was operated in the data-dependent acquisition mode MS spectra scanning from m/z 350–1550 at 120,000 resolution with AGC target of 5e5. The “top speed” acquisition method mode (3 s cycle time) on the most intense precursor was used whereby peptide ions with charge states ≥2–5 were isolated with isolation window of 1.6 m/z and fragmented with high energy collision (HCD) mode with stepped collision energy of 30 ± 5%. Fragment ion spectra were acquired in Orbitrap at 15,000 resolution. Dynamic exclusion was activated for 30 s.
Protein identification and quantification
MS data from DDA profiling were processed using Maxquant v1.5.5.1. MS/MS spectra were searched against the Uniprot human reference proteome FASTA file (downloaded on 21 February 2017). Digestion mode was set as trypsin. Label-free quantification (LFQ) was applied. Carbamidomethyl cysteine was set as a fixed modification; oxidation of methionine, phosphorylation of serine, threonine and tyrosine were considered variable modifications. False discovery rate (FDR) was set to 0.01.
Data analysis
Statistical analysis was performed using the Perseus package (Max Planck Institute of Biochemistry)113. A localization probability of ≥0.75 to a single amino acid residue for phosphopeptide was applied and parameters were set as default. Differential expression between groups was analyzed by two-sample t-test with the significance cut-off being p < 0.05. Pathway enrichment analysis was performed using the Ingenuity Pathway Analysis (IPA) package (QIAGEN Inc., https://digitalinsights.qiagen.com/IPA) using default settings.
Cell cycle analysis
T47D cells (150,000 cells/well) were plated in 6-well plates and treated as indicated. One hour before the end of treatment, cells were pulsed with 1:100 BrdU (Invitrogen #00-0103). For cell cycle analysis, cells were trypsinised, pelleted by centrifugation and ice-cold 70% ethanol was added dropwise into each sample while on gentle vortex. After fixing on ice for 1 h, cells were washed twice in PBS at 500 × g for 10 min. 2 N HCl/0.5% Triton X-100 was added dropwise to permeabilise and denature the DNA at RT for 30 min. The pH was neutralized with 0.1 M sodium tetraborate decahydrate NaB4O7 solution (pH8.5) and samples washed in 1%BSA/PBS. Cells were labeled with anti-BrdU primary antibodies (abcam #ab6326) and secondary antibodies in 1% BSA/0.2% Tween-20 in PBS. Samples were resuspended in propidium iodide/RNase solution. Cell cycle profiles were analyzed using a BD LSRFortessaTM X-20 flow cytometer. Raw data were analyzed using FlowJo 10.3.0 software package.
Quantitative reverse-transcription PCR
Cells were lysed in TRI reagent (Thermo Fisher Scientific, #AM9738) and total RNA extracted using Direct-zol RNA Miniprep Kits (Zymo Research, #R2050). RNA was reverse-transcribed into cDNA with QuantiTect Reverse Transcription Kit (QIAGEN). qPCR was performed in 2X QuantiNova STBR Green PCR Master Mix in CFX384 Touch Real-Time PCR Detection System (Bio-Rad). Ct values were determined in Bio-Rad CFX Manager v3.1 software package and the relative quantification was derived using the ΔΔCt method.
β-galactosidase cell senescence assay
T47D cells (25,000 cells/well) were plated on collagen-coated glass coverslips (10 μg/cm2) in 24-well plates overnight and treated as indicated. Drugs were pulsed every 2 days and at the end of treatments, cells were washed with 1X PBS and processed according to the senescence β-galactosidase (β-gal) staining kit (Cell Signaling Technologies, #9860). Cells were then counter-stained with DAPI (1 μg/ml) and mounted in 70% glycerol on glass slides. Olympus dotSlide digital virtual microscope was used to acquire DAPI and bright-field images. Total cell number (DAPI) and β-gal positive cells were quantified using Fiji software package.
γH2AX and 53BP1 staining
T47D cells (200,000 cells/well) were plated in 6-well plates and treated as indicated. At the end of each treatment, cells were treated with KaryoMAX Colcemid at 10 mg/ml for 1 h prior to harvest. Cells were subjected to hypotonic treatment in 0.075 M KCl (room temperature for 5 min), cyto-spun onto slides, and incubated in ice-cold KCM buffer (120 mM KCl, 10 mM Tris-HCl pH 7.5, 20 mM NaCl, 0.5 mM EDTA, 0.1% (v/v) Triton X-100 and protease inhibitor) for 5 min. Slides were incubated in ice-cold KCM extraction buffer (KCM and 0.4% Triton X-100) for 5 min, followed by an incubation in ice-cold KCM blocking buffer (KCM, 2% BSA, protease inhibitor and AEBSF) for another 5 min. Slides were incubated in anti-centromere human CREST (calcinosis, Raynaud phenomenon, esophageal dysmotility, sclerodactyly, and telangiectasia) and anti-phospho-histone H2A.X (Ser139) (Merck Millipore JBW301), or anti-53BP1 (ab21083) and secondary antibodies for 1 h at 37 °C in KCM block buffer. After antibody incubation, slides were washed three times with ice-cold KCM, and then fixed in 4% (v/v) formaldehyde (in KCM) and mounted with DAPI in Vectashield media. Images were collected using a Zeiss imager M2 fluorescence microscope linked to an AxioCam MRm CCD camera system. Image analysis was performed in Fiji software package. DAPI stain was used to create a mask for nuclei. Integrated fluorescence intensity of γH2AX per nucleus and 53BP1 per nucleus was quantified.
Cell death assay
T47D cells (25,000 cells/well in 24-well plate) were incubated with propidium iodide (PI) (1 mg/ml) (Thermo Fisher Scientific, P3566) and Hoechst 33342 solution (0.5 mg/ml) (Thermo Fisher Scientific, #62249) in a cell culture incubator for 30 min. Multiple fields per wells were imaged using a Leica DMi8 inverted microscope at ×10 magnification. Fiji software package was used to quantify the number of PI+ cells and the total cell number per field.
p21 cellular localization
T47D cells were grown on collagen-coated cover slips (25,000 cells/well in a 24-well plate) and treated as indicated. Cells were then fixed in 4% formaldehyde for 15 min and washed with 1X PBS three times. Permeabilisation and blocking step was done by incubating cells in 5% normal goat serum with 0.3% Triton-X 100 for 1 hr at RT. Standard IF protocol was used to probe for p21 using the rabbit mAb CST#2947. Cells were stained with DAPI and Wheat Germ Agglutinin-Alexa Fluor 555 for nuclear and whole cell segmentation, respectively. Multiple fields per well were imaged using a Leica DMi8 microscope at 20X magnification. Integrated intensity of p21 localization in nuclei and whole cells was quantified using the CellProfiler software package.
CellTiter-Glo assay
The dose-response of T47D cell lines to small molecule inhibitors was assayed using the CellTiter-Glo® 3D-Cell Viability assay (Promega, #G9681) according to the manufacturer’s instructions. Briefly, 5000 cells/well were plated in a 96-well plate and treated with increasing concentrations of inhibitors. At the end of each treatment, culture media was removed and plain RPMI media was added to each well. An equal volume of CellTiter reagent was added to the wells and plate/s shaken in a PHERAstar FSX for 5 min. Plates were then incubated in the dark for 30 min on a platform rocker, at the end of which contents were transferred into white OptiPlates and the integrated luminescence signal detected using a PHERAstar FSX.
Simulation of drugs combinations and drugs synergy
Drug synergy was computed based on coefficients of drug interaction (CDI) metric17,114: CDI = E12/(E1 × E2), where E12 is the normalized effect induced by drug 1 combined with drug 2, on a specific biological readout; E1 and E2 represent the effect of a single drug. CDI values lower than 1 indicate synergistic effects, CDI values equal or higher than 1 indicate additive or antagonistic effects, respectively. The degree of synergism versus antagonism is indicated by how small or large CDI values are compared to 1.
Patient survival analysis
mRNA expression, mutation profile and associated overall survival (OS) data from 2509 breast cancer patients (METABRIC)115 were downloaded from cBioPortal (https://www.cbioportal.org/). Breast cancer patients were classified based on CDKN1A and CCND1 expressions into three groups having either low, normal, or high expression levels. These were associated with the PIK3CA mutational status defined as either mutated or wildtype. Combination sub-groups were derived as such: (i) PIK3CA mutation and CDKN1A (or CCND1) high; (ii) PIK3CA mutation and CDKN1A (or CCND1) low; (iii) PIK3CA wildtype and CDKN1A (or CCND1) high; (iv) PIK3CA wildtype and CDKN1A (or CCND1) low. OS between sub-groups were subsequently performed using R package ‘survival’, with p < 0.05 considered significant.
List of antibodies with catalog numbers and dilutions:
Rabbit monoclonal anti-Phospho-Akt (Ser473) (clone D9E) 1:1000 dilution | Cell Signaling Technology | Cat# 4060; RRID:AB_2315049 |
Rabbit monoclonal anti-Phospho-Akt (Thr308) (clone D25E6) 1:1000 dilution | Cell Signaling Technology | Cat# 13038; RRID:AB_2629447 |
Rabbit monoclonal anti- Phospho-S6 Ribosomal Protein (Ser240/244) (clone D68F8) 1:2000 dilution | Cell Signaling Technology | Cat# 5364, RRID:AB_10694233 |
Rabbit monoclonal anti-S6 Ribosomal Protein (clone 5G10) 1:2000 dilution | Cell Signaling Technology | Cat# 2217; RRID:AB_331355 |
Mouse monoclonal anti-Actin (clone AC-40) 1:5000 dilution | Sigma-Aldrich | Cat# A3853; RRID:AB_262137 |
Rabbit monoclonal anti-Phospho4E-BP1 (Thr37/46) (236B4) 1:1000 dilution | Cell Signaling Technology | Cat# 2855; RRID:AB_560835 |
Rabbit monoclonal anti-Akt (pan) (clone 11E7) 1:1000 dilution | Cell Signaling Technology | Cat# 4685; RRID:AB_2225340 |
Rabbit monoclonal anti-Phospho Rb (Ser807/811) 1:2000 dilution | Cell Signaling Technology | Cat# 8516; RRID:AB_11178658 |
Rabbit monoclonal anti-Phosphop44/42 MAPK (Erk1/2) (Thr202/Tyr204) 1:1000 dilution | Cell Signaling Technology | Cat# 4370; RRID:AB_2315112 |
p44/42 MAPK (Erk1/2) 1:1000 dilution | Cell Signaling Technology | Cat# 4696; RRID: AB_390780 |
Rabbit polyclonal anti-Cyclin D1 1:1000 dilution | Cell Signaling Technology | Cat# 2922; RRID:AB_2228523 |
Mouse monoclonal anti-Cyclin A (clone AT10.2) 1:1000 dilution | Santa Cruz Biotechnology | Cat# sc-53227; RRID:AB_782329 |
Rabbit monoclonal anti-CDK4 (clone D9G3E) 1:1000 dilution | Cell Signaling Technology | Cat# 12790; RRID:AB_2631166 |
Mouse monoclonal anti-CDK6 (clone DCS22) 1:1000 dilution | Cell Signaling Technology | Cat# 3136; RRID:AB_2229289 |
Rabbit monoclonal anti-CDK2 (clone 78B2) 1:1000 dilution | Cell Signaling Technology | Cat# 2546; RRID:AB_2276129 |
Rabbit monoclonal anti-p21 Waf1/Cip1 (clone 12D1) 1:1000 dilution | Cell Signaling Technology | Cat# 2947 RRID:AB_823586 |
Mouse monoclonal anti-p18 INK4C (clone DCS118) 1:1000 dilution | Cell Signaling Technology | Cat# 2896; RRID:AB_331203 |
Rabbit monoclonal anti-p27 Kip1 (clone D69C12) 1:1000 dilution | Cell Signaling Technology | Cat# 3686; RRID:AB_2077850 |
Rabbit monoclonal anti-Phospho-Chk1 (Ser345) (clone 133D3) 1:1000 dilution | Cell Signaling Technology | Cat# 2348; RRID:AB_331212 |
Mouse monoclonal anti-PCNA (clone PC10) 1:1000 dilution | Cell Signaling Technology | Cat#2586; RRID:AB_2160343 |
Rabbit monoclonal anti-CDKN2A/p16INK4a (clone EPR1473) 1:1000 dilution | Abcam | Cat# ab108349; RRID:AB_10858268 |
Mouse monoclonal anti-p53 (clone 1C12) 1:1000 dilution | Cell Signaling Technology | Cat# 2524; RRID:AB_331743 |
Rabbit polyclonal anti-53BP1 1:500 dilution | Abcam | Cat# ab21083 RRID:AB_722496 |
Mouse monoclonal anti-phospho-Histone H2A.X (Ser139) (clone JBW301) 1:1000 dilution | Millipore | Cat# 05-636, RRID:AB_309864 |
Rabbit monoclonal anti-phospho-NDRG1 (Thr346) (D98G11) XP® 1:500 dilution | Cell Signaling Technology | Cat# 5482; RRID:AB_10693451 |
Rabbit monoclonal anti-hospho-SGK3 (Thr320) (D30E6) 1:500 dilution | Cell Signaling Technology | Cat# 5642; RRID: AB_10694357 |
Uncropped scans of the most important blots and gating strategy for Fig. 3d are provided as Supplementary Figs. 7–9 in the Supplementary Information File.
Reporting summary
Further information on research design is available in the Nature Research Reporting Summary linked to this article.
Data availability
Proteomics data have been deposited to the ProteomeXchange Consortium via PRIDE1 partner repository with the dataset identifier PXD033956.
Code availability
All the codes for modeling have been deposited in Github and can be accessed at: https://github.com/NguyenLabNetworkModeling/Integrated-PI3K-Signaling-Network-model.
References
Csolle, M. P., Ooms, L. M., Papa, A. & Mitchell, C. A. PTEN and other PtdIns(3,4,5)P3 lipid phosphatases in breast cancer. Int. J. Mol. Sci. 21, 9189 (2020).
Manning, B. D. & Toker, A. AKT/PKB signaling: navigating the network. Cell 169, 381–405 (2017).
Vanhaesebroeck, B., Perry, M. W. D., Brown, J. R., Andre, F. & Okkenhaug, K. PI3K inhibitors are finally coming of age. Nat. Rev. Drug Discov. 20, 741–769 (2021).
Andre, F. et al. Alpelisib for PIK3CA-mutated, hormone receptor-positive advanced breast cancer. N. Engl. J. Med. 380, 1929–1940 (2019).
Yip, H. Y. K. & Papa, A. Signaling pathways in cancer: therapeutic targets, combinatorial treatments, and new developments. Cells 10, 659 (2021).
Yip, H. Y. K. et al. Control of glucocorticoid receptor levels by PTEN establishes a failsafe mechanism for tumor suppression. Mol. Cell 80, 279–295.e8 (2020).
Elkabets, M. et al. mTORC1 inhibition is required for sensitivity to PI3K p110alpha inhibitors in PIK3CA-mutant breast cancer. Sci. Transl. Med. 5, 196ra199 (2013).
Leroy, C. et al. Activation of IGF1R/p110beta/AKT/mTOR confers resistance to alpha-specific PI3K inhibition. Breast Cancer Res. 18, 41 (2016).
Juric, D. et al. Convergent loss of PTEN leads to clinical resistance to a PI(3)Kalpha inhibitor. Nature 518, 240–244 (2015).
Castel, P. et al. PDK1-SGK1 signaling sustains AKT-independent mTORC1 activation and confers resistance to PI3Kalpha inhibition. Cancer Cell 30, 229–242 (2016).
Vora, S. R. et al. CDK 4/6 inhibitors sensitize PIK3CA mutant breast cancer to PI3K inhibitors. Cancer Cell 26, 136–149 (2014).
Tyson, J. J., Laomettachit, T. & Kraikivski, P. Modeling the dynamic behavior of biochemical regulatory networks. J. Theor. Biol. 462, 514–527 (2019).
Costa, C. et al. Measurement of PIP3 levels reveals an unexpected role for p110beta in early adaptive responses to p110alpha-specific inhibitors in luminal breast cancer. Cancer Cell 27, 97–108 (2015).
Raue, A., Karlsson, J., Saccomani, M. P., Jirstrand, M. & Timmer, J. Comparison of approaches for parameter identifiability analysis of biological systems. Bioinformatics 30, 1440–1448 (2014).
Neve, R. M., Holbro, T. & Hynes, N. E. Distinct roles for phosphoinositide 3-kinase, mitogen-activated protein kinase and p38 MAPK in mediating cell cycle progression of breast cancer cells. Oncogene 21, 4567–4576 (2002).
Villaverde, A. F., Pathirana, D., Frohlich, F., Hasenauer, J. & Banga, J. R. A protocol for dynamic model calibration. Brief. Bioinform. 23, bbab387 (2022).
Tsherniak, A. et al. Defining a cancer dependency map. Cell 170, 564–576.e16 (2017).
Kramer, A., Green, J., Pollard, J. Jr. & Tugendreich, S. Causal analysis approaches in Ingenuity Pathway Analysis. Bioinformatics 30, 523–530 (2014).
Sherr, C. J. & Roberts, J. M. CDK inhibitors: positive and negative regulators of G1-phase progression. Genes Dev. 13, 1501–1512 (1999).
Abbas, T. & Dutta, A. p21 in cancer: intricate networks and multiple activities. Nat. Rev. Cancer 9, 400–414 (2009).
Garrett, M. D. & Collins, I. Anticancer therapy with checkpoint inhibitors: what, where and when? Trends Pharmacol. Sci. 32, 308–316 (2011).
Galanos, P. et al. Chronic p53-independent p21 expression causes genomic instability by deregulating replication licensing. Nat. Cell Biol. 18, 777–789 (2016).
Wang, N. et al. The landscape of PDK1 in breast cancer. Cancers 14, 811 (2022).
Vasudevan, K. M. et al. AKT-independent signaling downstream of oncogenic PIK3CA mutations in human cancer. Cancer Cell 16, 21–32 (2009).
Turner, N. C., Neven, P., Loibl, S. & Andre, F. Advances in the treatment of advanced oestrogen-receptor-positive breast cancer. Lancet 389, 2403–2414 (2017).
Viale, A. et al. Cell-cycle restriction limits DNA damage and maintains self-renewal of leukaemia stem cells. Nature 457, 51–56 (2009).
Insinga, A. et al. DNA damage in stem cells activates p21, inhibits p53, and induces symmetric self-renewing divisions. Proc. Natl Acad. Sci. USA 110, 3931–3936 (2013).
Cayrol, C., Knibiehler, M. & Ducommun, B. p21 binding to PCNA causes G1 and G2 cell cycle arrest in p53-deficient cells. Oncogene 16, 311–320 (1998).
Prasanna, P. G. et al. Therapy-induced senescence: opportunities to improve anticancer therapy. J. Natl Cancer Inst. 113, 1285–1298 (2021).
Ewald, J. A., Desotelle, J. A., Wilding, G. & Jarrard, D. F. Therapy-induced senescence in cancer. J. Natl Cancer Inst. 102, 1536–1546 (2010).
Collado, M. & Serrano, M. Senescence in tumours: evidence from mice and humans. Nat. Rev. Cancer 10, 51–57 (2010).
Juvekar, A. et al. Phosphoinositide 3-kinase inhibitors induce DNA damage through nucleoside depletion. Proc. Natl Acad. Sci. USA 113, E4338–E4347 (2016).
Milanovic, M. et al. Senescence-associated reprogramming promotes cancer stemness. Nature 553, 96–100 (2018).
Cheng, X. et al. Breast cancer mutations HER2V777L and PIK3CAH1047R activate the p21-CDK4/6-Cyclin D1 axis to drive tumorigenesis and drug resistance. Cancer Res. 83, 2839–2857 (2023).
Sorensen, C. S. et al. The cell-cycle checkpoint kinase Chk1 is required for mammalian homologous recombination repair. Nat. Cell Biol. 7, 195–201 (2005).
Petermann, E., Woodcock, M. & Helleday, T. Chk1 promotes replication fork progression by controlling replication initiation. Proc. Natl Acad. Sci. USA 107, 16090–16095 (2010).
Chopra, S. S. et al. Torin2 exploits replication and checkpoint vulnerabilities to cause death of PI3K-activated triple-negative breast cancer cells. Cell Syst. 10, 66–81.e11 (2020).
Huang, T. T. et al. Targeting the PI3K/mTOR pathway augments CHK1 inhibitor-induced replication stress and antitumor activity in high-grade serous ovarian cancer. Cancer Res. 80, 5380–5392 (2020).
Llanos, S., Garcia-Pedrero, J. M., Morgado-Palacin, L., Rodrigo, J. P. & Serrano, M. Stabilization of p21 by mTORC1/4E-BP1 predicts clinical outcome of head and neck cancers. Nat. Commun. 7, 10438 (2016).
Hoxhaj, G. & Manning, B. D. The PI3K-AKT network at the interface of oncogenic signalling and cancer metabolism. Nat. Rev. Cancer 20, 74–88 (2020).
Ghomlaghi, M., Hart, A., Hoang, N., Shin, S. & Nguyen, L. K. Feedback, crosstalk and competition: ingredients for emergent non-linear behaviour in the PI3K/mTOR signalling network. Int. J. Mol. Sci. 22, 6944 (2021).
Leroy, C. et al. Activation of IGF1R/p110β/AKT/mTOR confers resistance to α-specific PI3K inhibition. Breast Cancer Res. 18, 41 (2016).
Zorea, J. et al. IGF1R upregulation confers resistance to isoform-specific inhibitors of PI3K in PIK3CA-driven ovarian cancer. Cell Death Dis. 9, 944 (2018).
Chakrabarty, A., Sánchez, V., Kuba, M. G., Rinehart, C. & Arteaga, C. L. Feedback upregulation of HER3 (ErbB3) expression and activity attenuates antitumor effect of PI3K inhibitors. Proc. Natl Acad. Sci. USA 109, 2718–2723 (2012).
Jeong, H. et al. Neuregulin-1 induces cancer stem cell characteristics in breast cancer cell lines. Oncol. Rep. 32, 1218–1224 (2014).
Tzahar, E. et al. A hierarchical network of interreceptor interactions determines signal transduction by Neu differentiation factor/neuregulin and epidermal growth factor. Mol. Cell. Biol. 16, 5276–5287 (1996).
Nakanishi, Y. et al. Activating mutations in PIK3CB confer resistance to PI3K inhibition and define a novel oncogenic role for p110β. Cancer Res. 76, 1193–1203 (2016).
Castel, P. et al. PDK1-SGK1 signaling sustains AKT-independent mTORC1 activation and confers resistance to PI3Kα inhibition. Cancer Cell 30, 229–242 (2016).
Serra, V. et al. PI3K inhibition results in enhanced HER signaling and acquired ERK dependency in HER2-overexpressing breast cancer. Oncogene 30, 2547–2557 (2011).
De Benedetti, A. & Graff, J. R. eIF-4E expression and its role in malignancies and metastases. Oncogene 23, 3189–3199 (2004).
Lin, C.-J., Malina, A. & Pelletier, J. c-Myc and eIF4F constitute a feedforward loop that regulates cell growth: implications for anticancer therapy. Cancer Res. 69, 7491–7494 (2009).
Haberichter, T. et al. A systems biology dynamical model of mammalian G1 cell cycle progression. Mol. Syst. Biol. 3, 84 (2007).
Calzone, L., Gelay, A., Zinovyev, A., Radvanyi, F. & Barillot, E. A comprehensive modular map of molecular interactions in RB/E2F pathway. Mol. Syst. Biol. 4, 173 (2008).
Yao, G. Modelling mammalian cellular quiescence. Interface Focus 4, 20130074 (2014).
Bottazzi, M. E., Zhu, X., Böhmer, R. M. & Assoian, R. K. Regulation of p21(cip1) expression by growth factors and the extracellular matrix reveals a role for transient ERK activity in G1 phase. J. Cell Biol. 146, 1255–1264 (1999).
Li, Y., Dowbenko, D. & Lasky, L. A. AKT/PKB phosphorylation of p21Cip/WAF1 enhances protein stability of p21Cip/WAF1 and promotes cell survival. J. Biol. Chem. 277, 11352–11361 (2002).
Nguyen, L. K. & Kholodenko, B. N. Feedback regulation in cell signalling: lessons for cancer therapeutics. Semin. Cell Dev. Biol. 50, 85–94 (2016).
Zhang, J. et al. Inhibition of Rb phosphorylation leads to mTORC2-mediated activation of Akt. Mol. Cell 62, 929–942 (2016).
Goel, S. et al. Overcoming therapeutic resistance in HER2-positive breast cancers with CDK4/6 inhibitors. Cancer Cell 29, 255–269 (2016).
Copps, K. D. & White, M. F. Regulation of insulin sensitivity by serine/threonine phosphorylation of insulin receptor substrate proteins IRS1 and IRS2. Diabetologia 55, 2565–2582 (2012).
Manning, B. D. Balancing Akt with S6K: implications for both metabolic diseases and tumorigenesis. J. Cell Biol. 167, 399–403 (2004).
Yoneyama, Y. et al. Serine phosphorylation by mTORC1 promotes IRS-1 degradation through SCFβ-TRCP E3 ubiquitin ligase. iScience 5, 1–18 (2018).
Cantley, L. C. The phosphoinositide 3-kinase pathway. Science 296, 1655–1657 (2002).
Kiyatkin, A. et al. Scaffolding protein Grb2-associated binder 1 sustains epidermal growth factor-induced mitogenic and survival signaling by multiple positive feedback loops. J. Biol. Chem. 281, 19925–19938 (2006).
Wang, W., Xu, S., Yin, M. & Jin, Z. G. Essential roles of Gab1 tyrosine phosphorylation in growth factor-mediated signaling and angiogenesis. Int. J. Cardiol. 181, 180–184 (2015).
Welch, H. C. et al. P-Rex1, a PtdIns(3,4,5)P3- and Gbg-regulated guanine-nucleotide exchange factor for Rac. Cell 108, 809–821 (2002).
Hill, K. et al. Regulation of P-Rex1 by phosphatidylinositol (3,4,5)-trisphosphate and Gbetagamma subunits. J. Biol. Chem. 280, 4166–4173 (2005).
Srijakotre, N. et al. P-Rex1 and P-Rex2 RacGEFs and cancer. Biochem. Soc. Trans. 45, 963–977 (2017).
Fritsch, R. et al. RAS and RHO families of GTPases directly regulate distinct phosphoinositide 3-kinase isoforms. Cell 153, 1050–1063 (2013).
Knaus, U. G., Wang, Y., Reilly, A. M., Warnock, D. & Jackson, J. H. Structural requirements for PAK activation by Rac GTPases. J. Biol. Chem. 273, 21512–21518 (1998).
Baker, N. M., Yee Chow, H., Chernoff, J. & Der, C. J. Molecular pathways: targeting RAC-p21-activated serine-threonine kinase signaling in RAS-driven cancers. Clin. Cancer Res. 20, 4740–4746 (2014).
Sosa, M. S. et al. Identification of the Rac-GEF P-Rex1 as an essential mediator of ErbB signaling in breast cancer. Mol. Cell 40, 877–892 (2010).
Liu, H.-J. et al. PREX1 Rac-GEF activity promotes breast cancer cell proliferation and tumor growth via activation of extracellular-signal-regulated kinase 1/2 (ERK1/2) signaling. J. Biol. Chem. 291, 17258–17270 (2016).
Birtwistle, M. R. & Kolch, W. Biology using engineering tools: the negative feedback amplifier. Cell Cycle 10, 2069–2076 (2011).
Wang, X., Hu, S. & Liu, L. Phosphorylation and acetylation modifications of FOXO3a: independently or synergistically? Oncol. Lett. 13, 2867–2872 (2017).
Brunet, A. et al. Protein kinase SGK mediates survival signals by phosphorylating the forkhead transcription factor FKHRL1 (FOXO3a). Mol. Cell. Biol. 21, 952–965 (2001).
Bosch, A. et al. PI3K inhibition results in enhanced estrogen receptor function and dependence in hormone receptor–positive breast cancer. Sci. Transl. Med. 7, 283ra251 (2015).
Malinen, M. et al. Proto-oncogene PIM-1 is a novel estrogen receptor target associating with high grade breast tumors. Mol. Cell. Endocrinol. 365, 270–276 (2013).
Wang, C. et al. Estrogen induces c-myc gene expression via an upstream enhancer activated by the estrogen receptor and the AP-1 transcription factor. Mol. Endocrinol. 25, 1527–1538 (2011).
Xu, J. et al. SGK3 is associated with estrogen receptor expression in breast cancer. Breast Cancer Res. Treat. 134, 531–541 (2012).
Wang, Y. et al. SGK3 is an estrogen-inducible kinase promoting estrogen-mediated survival of breast cancer cells. Mol. Endocrinol. 25, 72–82 (2011).
Thomas, R. S., Sarwar, N., Phoenix, F., Coombes, R. C. & Ali, S. Phosphorylation at serines 104 and 106 by Erk1/2 MAPK is important for estrogen receptor-α activity. J. Mol. Endocrinol. 40, 173–184 (2008).
Verma, N. et al. Targeting of PYK2 synergizes with EGFR antagonists in basal-like TNBC and circumvents HER3-associated resistance via the NEDD4-NDRG1 axis. Cancer Res. 77, 86–99 (2017).
Kovacevic, Z. et al. The metastasis suppressor, N-MYC downstream-regulated gene-1 (NDRG1), down-regulates the ErbB family of receptors to inhibit downstream oncogenic signaling pathways. J. Biol. Chem. 291, 1029–1052 (2016).
Murray, J. T. et al. Exploitation of KESTREL to identify NDRG family members as physiological substrates for SGK1 and GSK3. Biochem. J. 384, 477–488 (2004).
Gasser, J. A. et al. SGK3 mediates INPP4B-dependent PI3K signaling in breast cancer. Mol. Cell 56, 595–607 (2014).
Moelling, K., Schad, K., Bosse, M., Zimmermann, S. & Schweneker, M. Regulation of Raf-Akt cross-talk. J. Biol. Chem. 277, 31099–31106 (2002).
Zimmermann, S. & Moelling, K. Phosphorylation and regulation of Raf by Akt (protein kinase B). Science 286, 1741–1744 (1999).
Lehr, S. et al. Identification of major ERK-related phosphorylation sites in Gab1. Biochemistry 43, 12133–12140 (2004).
Yu, C. F., Liu, Z. X. & Cantley, L. G. ERK negatively regulates the epidermal growth factor-mediated interaction of Gab1 and the phosphatidylinositol 3-kinase. J. Biol. Chem. 277, 19382–19388 (2002).
Zhang, X. et al. Extracellular signal-regulated kinases 1 and 2 phosphorylate Gab2 to promote a negative-feedback loop that attenuates phosphoinositide 3-kinase/Akt signaling. Mol. Cell Biol. 37, e00357-16 (2017).
Ashyraliyev, M., Fomekong-Nanfack, Y., Kaandorp, J. A. & Blom, J. G. Systems biology: parameter estimation for biochemical models. FEBS J. 276, 886–902 (2009).
Raue, A. et al. Lessons learned from quantitative dynamical modeling in systems biology. PLoS ONE 8, e74335 (2013).
Raue, A. et al. Structural and practical identifiability analysis of partially observed dynamical models by exploiting the profile likelihood. Bioinformatics 25, 1923–1929 (2009).
Ghomlaghi, M., Yang, G., Shin, S.-Y., James, D. E. & Nguyen, L. K. Dynamic modelling of the PI3K/MTOR signalling network uncovers biphasic dependence of mTORC1 activity on the mTORC2 subunit SIN1. PLoS Comput. Biol. 17, e1008513 (2021).
Reali, F., Priami, C. & Marchetti, L. Optimization algorithms for computational systems biology. Front. Appl. Math. Stat. 3 https://doi.org/10.3389/fams.2017.00006 (2017).
Man, K. F., Tang, K. S. & Kwong, S. Genetic algorithms: concepts and applications [in engineering design]. IEEE Trans. Ind. Electron. 43, 519–534 (1996).
Shin, S. Y. et al. The switching role of b-adrenergic receptor signalling in cell survival or death decision of cardiomyocytes. Nat. Commun. 5, 5777 (2014).
Frenzel, J. F. Genetic algorithms. IEEE Potentials 12, 21–24 (1993).
Villaverde, A. F., Pathirana, D., Fröhlich, F., Hasenauer, J. & Banga, J. R. A protocol for dynamic model calibration. Brief. Bioinform. 23 https://doi.org/10.1093/bib/bbab387 (2021).
Shin, S.-Y., Müller, A.-K., Verma, N., Lev, S. & Nguyen, L. K. Systems modelling of the EGFR-PYK2-c-Met interaction network predicts and prioritizes synergistic drug combinations for triple-negative breast cancer. PLoS Comput. Biol. 14, e1006192 (2018).
Fey, D. et al. Signaling pathway models as biomarkers: patient-specific simulations of JNK activity predict the survival of neuroblastoma patients. Sci. Signal. 8, ra130 (2015).
Pabla, N., Bhatt, K. & Dong, Z. Checkpoint kinase 1 (Chk1)-short is a splice variant and endogenous inhibitor of Chk1 that regulates cell cycle and DNA damage checkpoints. Proc. Natl Acad. Sci. USA 109, 197–202 (2012).
Bian, L., Meng, Y., Zhang, M. & Li, D. MRE11-RAD50-NBS1 complex alterations and DNA damage response: implications for cancer treatment. Mol. Cancer 18, 169 (2019).
Nowsheen, S. & Yang, E. S. The intersection between DNA damage response and cell death pathways. Exp. Oncol. 34, 243–254 (2012).
Wang, X. et al. A positive role for c-Abl in Atm and Atr activation in DNA damage response. Cell Death Differ. 18, 5–15 (2011).
Lin, W. C., Lin, F. T. & Nevins, J. R. Selective induction of E2F1 in response to DNA damage, mediated by ATM-dependent phosphorylation. Genes Dev. 15, 1833–1844 (2001).
Aki, T. & Uemura, K. Cell death and survival pathways involving ATM protein kinase. Genes 12, 1581 (2021).
Liu, Q. et al. Chk1 is an essential kinase that is regulated by Atr and required for the G(2)/M DNA damage checkpoint. Genes Dev. 14, 1448–1459 (2000).
Bartek, J. & Lukas, J. Chk1 and Chk2 kinases in checkpoint control and cancer. Cancer Cell 3, 421–429 (2003).
Shen, T. & Huang, S. The role of Cdc25A in the regulation of cell proliferation and apoptosis. Anticancer Agents Med. Chem. 12, 631–639 (2012).
Christmann, M. & Kaina, B. Transcriptional regulation of human DNA repair genes following genotoxic stress: trigger mechanisms, inducible responses and genotoxic adaptation. Nucleic Acids Res. 41, 8403–8420 (2013).
Tyanova, S. et al. The Perseus computational platform for comprehensive analysis of (prote)omics data. Nat. Methods 13, 731–740 (2016).
Steiert, B., Raue, A., Timmer, J. & Kreutz, C. Experimental design for parameter estimation of gene regulatory networks. PLoS ONE 7, e40052 (2012).
Pereira, B. et al. The somatic mutation profiles of 2,433 breast cancers refines their genomic and transcriptomic landscapes. Nat. Commun. 7, 11479 (2016).
LaBaer, J. et al. New functional activities for the p21 family of CDK inhibitors. Genes Dev. 11, 847–862 (1997).
Acknowledgements
The authors are grateful to Robin M. Hobbs and to members of the Papa and Nguyen labs for their support. The authors acknowledge the Monash Biochemistry Imaging Facility, FlowCore, and Micro Imaging Platforms, and the Mass Spectrometry and Proteomics facility—Bio21 Institute, University of Melbourne. Figure 6g was generated with BioRender. The Novo Nordisk Foundation Center for Stem Cell Medicine, reNEW, is supported by a Novo Nordisk Foundation grant number NNF21CC0073729. L.K.N. and A.P. are supported by Victorian Cancer Agency Mid-Career Research Fellowships (MCRF18026 and MCRF20027). This work was supported by a NHMRC grant to A.P. (APP1100307) and in part by an IIRS-National Breast Cancer Foundation, and Love Your Sister (IIRS-20–094) to L.K.N.
Author information
Authors and Affiliations
Contributions
H.Y.K.Y., S.Y.S., L.K.N., and A.P. designed the study; H.Y.K.Y., S.Y.S., A.C. and A.P. performed experiments; S.Y.S., F.J.R., and C.S.A. contributed new reagents/analytic tools; H.Y.K.Y., S.Y.S., A.C., L.H.W., L.K.N., and A.P. analyzed data; L.K.N. and A.P. supervised the study. L.K.N. and A.P. wrote the paper. H.Y.K.Y. and S.Y.S. are co-first authors.
Corresponding authors
Ethics declarations
Competing interests
F.J.R. receives institutional support as a coinvestigator and is subcontracted by the Peter MacCallum Cancer Centre for an investigator initiated trial which receives funding support from Sanofi/Regeneron Pharmaceuticals.
Additional information
Publisher’s note Springer Nature remains neutral with regard to jurisdictional claims in published maps and institutional affiliations.
Rights and permissions
Open Access This article is licensed under a Creative Commons Attribution 4.0 International License, which permits use, sharing, adaptation, distribution and reproduction in any medium or format, as long as you give appropriate credit to the original author(s) and the source, provide a link to the Creative Commons license, and indicate if changes were made. The images or other third party material in this article are included in the article’s Creative Commons license, unless indicated otherwise in a credit line to the material. If material is not included in the article’s Creative Commons license and your intended use is not permitted by statutory regulation or exceeds the permitted use, you will need to obtain permission directly from the copyright holder. To view a copy of this license, visit http://creativecommons.org/licenses/by/4.0/.
About this article
Cite this article
Yip, H.Y.K., Shin, SY., Chee, A. et al. Integrative modeling uncovers p21-driven drug resistance and prioritizes therapies for PIK3CA-mutant breast cancer. npj Precis. Onc. 8, 20 (2024). https://doi.org/10.1038/s41698-024-00496-y
Received:
Accepted:
Published:
DOI: https://doi.org/10.1038/s41698-024-00496-y