I am running a simple isocratic Shimadzu HPLC system coupled to a fluorescence detector to detect and quantify biogenic amines from in vivo samples. But my results are not as expected and I'm having trouble identifying the the problems.

My current method:

Column: Supelco C18 reverse phase 250 x 4.6mm, 5uM pore size

Temperature: 45C

Flow rate: 1.5mL/minute,

Injector: manual injector, 20uL injection volume.

Detector: Fluorescence, Ex:280nM, Em:345nM

Mobile phase: (40:60) Methanol : 10mM Sodium acetate buffer (pH4.5)

My 3 analytes of interest, which are naturally fluorescent, are structurally similar: tryptamine (TA), N-methyltryptamine (NMT), and N,N-dimethyltryptamine (DMT). But when I inject standards of these compounds individually, I get unexpected results.

Tryptamine (which is the most polar of the three) elutes later than DMT (least polar), and it shows a very broad (5-6 minutes long) peak. By contrast, DMT gives a relatively sharp peak. When I run these three compounds on TLC silica plates with a polar mobile phase, tryptamine travels furthest, followed by NMT then DMT. So this brings up two questions, which are probably related:

  • Why might tryptamine be eluting later than dimethyltryptamine?
  • Why is there such drastic peak broadening with tryptamine, but not with DMT?

I have experimented with modifying the mobile phase (varying from 34-50% MeOH), modifying pH (from 3.5 - 6.0), modifying sodium acetate buffer concentration (from 10mM - 50mM), modifying Ex:Em detector settings, time constant/sensitivity detector settings, column replacement, injector volume, sample preparation (injecting in pure water vs. pure methanol vs. mobile phase), and others. None of these have really resolved my issues.

Could anyone provide any direction on other potential strategies for method improvement?

Thanks in advance.

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