-
- Posts: 8
- Joined: Tue Mar 04, 2008 6:29 pm
MP A is 0.88 g sodium 1 hexanesulfonate monohydrate, 950 mL 50 mM PO4 buffer and 50 mL CH3CN, pH 3.5
MP B is 0.88 g sodium 1 hexanesulfonate monohydrate, (125 mL 50 mM PO4 buffer + 125 mL water), and 750 mL CH3CN, pH 3.5.
We currently pH the mobile phase by aliquot-the pH probe does not touch the mobile phase. The wavelength is 210 nm and the gradient profile is 0% B at time zero to 100% B at 50 minutes, with 20 minutes reequilibration. The column called for in the method is a Kromasil 250 x 4.6, 5 um. The column heater is set at 35 degrees C.
The standard and sample is dissolved in methanol, and the standard has 6 components. However, our issue is with extraneous peaks in the methanol blank. Even using bottled water and high purity reagents and pH'ing the mobile phase by aliquot, we are getting around 25 peaks or so on each blank shot.
We've tried adjusting how the mobile phase is made, by pH'ing the buffer/pic reagent by aliquot then adding the CH3CN. And we've tried multiple columns. However, none of these things have cleaned up the baseline. It should be noted that most of our peaks are occurring later in the run, roughly 37 minutes onward.
If anyone has any ideas or suggestions, I'm more than ready to read them.
Thanks in advance.
