Hi everyone,

I recently performed Laurdan staining on live cells using a 10 µM working solution diluted in complete culture medium using Laurden from MCE (HY-D0080). I incubated the cells at 37°C for 1 hour, protected from light, and then fixed them with 4% paraformaldehyde for 15 minutes before imaging them on a confocal microscope. I used 440 nm and 488 nm excitation wavelengths, expecting to observe membrane labeling with yellow edges due to Laurdan’s spectral shift. However, the fluorescence signal was very weak, and the expected membrane outlining effect wasn’t clearly visible.

I’m wondering:

  • Is 1 hour of staining sufficient, or should I extend the incubation time?
  • Could fixation with paraformaldehyde be affecting the Laurdan signal?
  • Is there an optimal buffer or staining condition I should consider?
  • Could the weak signal be due to Laurdan's sensitivity to membrane phase rather than just presence?

Any advice or insight would be greatly appreciated. Thank you!

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