I am trying to differentiation human derived monocytes from blood into macrophages. I am culturing them in collagen coated plates (at 0.3 mg/mL) for 7 days. First I culture them for 6 days with 100 ng/mL M-CSF at 37 degrees +5%CO2 at a density of 1 million per mL per well. On day 6, I remove the media without disturbing the attached macrophages, spin my cells in the media and remove the supernatant. Then I resuspend them in 25 ng/mL of IFN-gamma (1O^6 IU/mL) and 1ug/mL of LPS. The media I used for my macrophages include RPMI +10% Human serum + 1% Penicilin/ streptomycin. By day 7, I remove the media, then wash with PBS and then add 500uL of warm 0.25% trypsin and try to remove the attached cells by pipetting vigorously as and incubate at 37 degrees for 5 minutes. Then I neutralize the trypsin using R10 and add everything to my media that was previously removed and spin everything. Usually my recovery barely gets as high as 20% and even by day 6 I already see a difference when comparing how the cells look on the microscope before and after changing the media. I do not know how to increase the recovery and have tried the same experiment at least 10 times where the recovery is usually around the same percentage of initial plated cells.