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

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