I'm following the protocol (https://www.frontiersin.org/articles/10.3389/fphar.2018.00071/full):

Cell differentiation was induced via a 6-h exposure to 185 ng/ml phorbol 12-myristate 13-acetate (PMA, Sigma–Aldrich) in DMSO. Cells were then polarized toward M1 or M2 phenotype by incubation for 48 more hours with INF-γ (20 ng/ml, Immunotools) and LPS (100 ng/ml, Sigma–Aldrich) or with IL-4 (20 ng/ml, Immunotools) and IL-13 (20 ng/ml, Immunotools), respectively (Tjiu et al., 2009; Maeß et al., 2014), still in the presence of PMA. Cells used for the resting condition were kept in the presence of PMA for 48 more hours in normal growth medium. CM were then prepared by keeping polarized as well as resting cells in serum-free RPMI without stimuli and no PMA for 72 more hours.

Basically, what I'm seeing are wells with M1 macrophages that dwindle in number over the 72 hours post-exposure to INF-γ and LPS. I'm not sure if this matters, but their distribution is typically only at the periphery of the well by the end of that time (images attached are of this area). Also, for some reason, their association (phagocytosis) with beads is lower than both M0 and M2. What could I be doing wrong?

Troubleshooting steps:

-Order fresh reagents & prepare new aliquots

-Tried another vendor

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