Edit: image uploaded
I've blotted for beta-actin on cell culture protein lysates many times but the beta-actin detection range was not between 37 - 50 kDa range but 25 - 37 kDa range each time.
Details of the western blot: lysates are from primary mixed glial cells lysed in RIPA + protease inhibitors and stored at -80. Protein concentrations are read by BCA assay.
I do SDS-PAGE in a 4-15% tris glycine mini-gel , run them at 200V for 30 min. After washing in TBS-T, I transfer onto a PVDF membrane with the semi-dry transfer and easily see the bands on the blot.
Then, I block with 1% skim milk (NFDM) in TBST for 1h RT, incubate in b-actin antibody (sigma 1:10000) overnight at 4 C. Then I incubate with anti-mouse HRP secondary 1h at RT.
I detect the blot by ECL reagent from GE for 5 minute and capture it.
I did trouble shooting many times. I also blot the membrane with B-actin before anything else but I got the same result. You think the problem is with the protein amount or something else? I load 20 ug of protein and then try with 10 ug of protein but I got the same result.
Thank you for your answers!