As previously described (Turn et al., 2020 (link)), unsynchronized cells were prepared for flow cytometry by trypsinizing the cells, taking up the cells in ice-cold phosphate-buffered saline (PBS), washing with ice-cold PBS, and fixing the cells with ice-cold 70% ethanol dropwise while simultaneously vortexing to reduce the risk of cell clumping. Both supernatant and adherent cells were collected to ensure that we had a full representation of the cell population. The day of flow cytometry, cells were spun down, washed with ice-cold phosphate citrate buffer (0.1 M citric acid in PBS, pH 7.8) two times, treated with RNase A for 15 min (100 µg/ml; Sigma; R5125), and treated with propidium iodide for 45 min (50 µg/ml; Sigma; P4170) to stain for DNA content. Cells were passed through a cell strainer and run on a FACSymphony A3. The G1 peak of WT cells was set at a 50,000 voltage for each run, and these settings were used to acquire all subsequent samples run that day to ensure that we accurately track 2N, 4N, and >4N peaks. At least 10,000 cells were collected per sample. FloJo software was used to plot data shown.