I'm checking the inhibition of amylase enzyme through starch hydrolysis. I will explain the protocol here:
Reagents:
PBS buffer- 20 mM, 6.9 pH, with 0.1 mM Cacl2 and 6.7 mM Nacl
40 U amylase
50 mg corn starch
0.5 mol/L sodium carbonate
Procedure:
1. 50 mg corn starch + inhabitor (3 different ratios- 1:0 (control), 1:2, 1:4, 1:6) + 9 ml PBS buffer incubated for 15 mins at 37 C with continuous mixing
2. After 15 mins, 1 ml amylase (1 ml containing 40 U) was added.
3. 300 uL of the mixture was withdrawn in predetermined time intervals (30 mins) - from 0th, 240th min to a centrifuge containing 1.2 ml sodium carbonate (stopping solution)
4. The sample mixtures were centrifuged for 5 mins at 11,800 g and 100 uL of supernatant was transferred to another centrifuge tube followed by the addition of 300 ul DNS reagent.
5. The tubes were boiled at 90 C for 5 mins.
A maltose std was also plotted. (45 mg in 50 ml DW) Concentrations taken- 0, 0.2 ml, 0.4 ml, 0.6 ml, 0.8 ml, 1 ml volume was made up to 2 ml and 1 ml DNS reagent was added.
My query:
DNS reagent reacted well with maltose std solutions and gave darker colours at higher concentrations of maltose.
However, there was no colour change for my samples.
Should I have gelatinized the starch samples before initiating the reaction?
Or the substrate concentration is too less for the enzyme?
Or more DNS reagent needs to be added to the mixture followed by 10 min of incubation in boiling water bath?
I tried adding 1 ml of DNS to 100 uL of the mixture and incubated at 100 C for 5 mins, still no colour change.