Hi,
I am performing a staining right now using three different antibodies for detection of some proteins in the hippocampus Dentate gyrus.
For the protocol, I am using two indirect antibodies (rat and rabbit) and one conjugated antibody (mouse), since the conjugated was the only one available for my staining purpose.
The conjugated AB worked in a test staining alone, incubated at 4°C Over night.
Using it together with the indirect Ab, I used following protocol:
1. Washing of brain slices
2. Blocking with NGS and triton-X
3. Incubation primary AB 4°C over night
4. Incubation 2nd AB 2h a room temp (host-species is goat)
5. Washing
6. Blocking again for 1h room temp with NGS
7. incubation of already conjugated mouse AB 4°C over night
8. Washing + Mounting
Using this protocol, the fluorescent signal that I am getting now from the conjugated Ab is dimmer (almost unrecognizable) and the background higher. I am using the AB in a dilution of 1:250. Both indirect antibodies are working perfectly as usual.
Should I increase the Blocking time or use a higher dilution?
I have to add: one of the indirect 1st Ab is anti-BrdU, so I have a pre incubation step with 2M HCL at the very beginning of the protocol.
Thank you very much for any ideas and help!
Best, Edna