PADM 5600 Chapter : Landons Project
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Experiment 1: Calculating Rate of Reaction
In this experiment you will calculate the rate of reaction of potassium iodide and hydrogen peroxide. The order of the reaction will also be determined.
Materials: 20 mL 3% Hydrogen peroxide, H2O2 | Stopwatch * You must provide *You must cut this piece of tubing into two, 12 inch pieces. (if you have not already done so). | |
Procedure
Preparation of Apparatus
Set up apparatus as shown in Figure 2. To do this, begin by labeling the Erlenmeyer Flasks as 1 and 2. The reaction will take place in Flask 1.
Fill Flask 2 approximately three quarters of the way full with water.
Press the 2-hole rubber stopper into the top of Flask 2. Place one three in. piece and one six in. piece of rigid tubing into each hole of the rubber stopper. This should create an airtight system.
Place the one-hole stopper on Flask 1, and fit the remaining 3 in. piece of rigid tubing in the stopper hole.
Connect Flask 1 and Flask 2 with the two, 12 in flexible tubing pieces. One piece should connect Flask 1 to Flask 2, and the second piece should connect Flask 2 to the graduated cylinder. The tubing which connects Flask 2 to the graduated cylinder should be positioned low enough to be immersed in the water in Flask 2.
Figure 2: Apparatus set-up. Note this is a sample set-up and is not drawn to scale. Your specific equipment may vary slightly. |
Part A: Preparation of Reactants
Pour five mL of the IKI solution into a 10 mL graduated cylinder.
Add five mL of distilled water to the graduated cylinder to bring the total volume to 10 mL. This is the 0.5% - 1.0% (diluted) IKI solution.
Pour 15 mL of 3% H2O2 solution into a 100 mL beaker.
Add five mL of distilled water to this beaker and mix with a stir rod. This is the 2.25% (diluted) H2O2 solution.
Part B: Performing the Reaction
Remove the stopper from Flask 1 and place five mL of the 3% (undiluted) H2O2 solution and 10 mL of the undiluted IKI solution provided into the flask. Immediately replace the stopper on the flask.
Note: At this point, you should select an extra beaker (any volume) from your lab kit to use as an supplemental collection container beaker for Step 6. You do not need to use the beaker yet, but keep it in close proximity.
Swirl Flask 1 until you observe a steady dripping of water going into the 10 mL graduated cylinder. This could take 3 - 5 minutes. Check for leaks in the tubing or system if water does not start rising up the plastic tubing coming from Flask 2 and traveling towards the graduated cylinder within one minute.
Stop swirling Flask 1 when you notice the steady flow of water droplets. When you stop, the water drop -rate will significantly decrease (to around one drop every 5 - 20 seconds) and could take a few minutes to stabilize. If a steady flow of drops of water does not occur within a few minutes, swirl Flask 1 for 1 more minute and check again. Repeat this process until there is a steady flow of drops of water after you have stopped swirling Flask 1.
Quickly empty liquid that has collected in the 10 mL graduated cylinder and replace the empty cylinder back under the flexible tubing.
Allow the flow of drops to become steady again. This could take 1 - 3 mL of water.
Start timing once the drop rate is steady and the volume of water collected is at a whole number (such as three mL). Record the time in Table 1 each time 2 mL of is water displaced. Continue taking data until you have at least 10 data points (20 mL displaced).
Note: Use the extra beaker (located in Part B: Step 1) to collect additional fluid when the volume of displaced water exceeds 10 mL.
Return the collected water from your 10 mL graduated cylinder to Flask 2. Ensure the seal is air tight.
Empty, clean and dry Flask 1 and the graduated cylinder.
Repeat Steps 1 - 8 for the following trial conditions: 5 mL 3% (undiluted) H2O2 mixed with 10 mL of 0.5%-1.0% IKI solution (placed in Flask 1); and, 5 mL of 2.25% H2O2 mixed with 10 mL of 1.0%-2.0% IKI solution (placed in Flask 1). Record the data in Table 2 and Table 3, respectively.
Note: Clean the graduated cylinder and extra collection beaker before it is used to measure any additional reagents for Trial 2 or Trial 3; and, before it is used for collecting the water from the reaction in the apparatus.
Use a graphing software program to make a graph of each trial. The graph should demonstrate the relationship formed between time vs. mL of water displaced.
Find and record the slope and the inverse slope for each trial.
Table 1: 10 mL Undiluted (1.0 -2.0%) IKI and 5 mL 3% H2O2 | |
mL water displaced | Time (seconds) |
2 | |
4 | |
6 | |
6 | |
8 | |
10 | |
12 | |
14 | |
16 | |
18 | |
20 | |
22 | |
Slope: | |
Inverse Slope: |
Table 2: 10 mL Diluted (0.5-1.0% IKI) and 5 mL 3% H2O2 | |
mL water displaced | Time (seconds) |
2 | |
4 | |
6 | |
6 | |
8 | |
10 | |
12 | |
14 | |
16 | |
18 | |
20 | |
22 | |
Slope: | |
Inverse Slope: |
Table 3: 10 mL Undiluted (1.0 -2.0%) IKI and 5 mL 2.25% H2O2 | |
mL water displaced | Time (seconds) |
2 | |
4 | |
6 | |
6 | |
8 | |
10 | |
12 | |
14 | |
16 | |
18 | |
20 | |
22 | |
Slope: | |
Inverse Slope: |
Calculations
Post-Lab Questions
1. Determine the order of the KI in this reaction.
2. Determine the order of the H2O2 in this reaction.
3. Calculate the rate law constant.
4. What is the overall rate law?
5. When finding the order of H2O2, why was Trial 1 and Trial 3 used?
6. When finding the order of KI, why was Trial 1 and Trial 2 used?
7. Research and identify some alternative catalysts that could be used to accelerate the decomposition of hydrogen peroxide. Evaluate these catalysts and determine which option is
yeast population dynamics
Procedure
1. Work in pairs on this lab, so 12 tubes per pair of students. And share a tube rack with one other pair of students
2. Turn on your spectrophotometer. It needs at least 15 minutes to warm up to give you good readings.
3. Add 5 mL of yeast extract solution (YECM) to each of 12 tubes. (The yeast extract provides vitamins and amino acids for yeast growth and will be the same for all cultures). The tubes should be labeled with your initials, treatment, and tube number. Tape or Parafilm down the lids of 3 tubes, and label them “CONTROL”.
Do not touch the insides of the tubes or lids! Try to keep these as sterile as possible!!
4. Add 50 mL live yeast culture to each of the remaining 9 tubes.
5. Add the varying volumes of sugar and/or ethanol using Table 1 below.
6. Use Parafilm to close the tops of each tube, making sure the Parafilm is tight and no air can get in, and label each tube with the following:
Amount of sugar added (mL) Amount of ethanol added (mL)
Name of your group Tube number
Table 1: setup yeast tubes (remember, 1 mL = 1000 mL) | ||||
Tube number | Yeast culture medium? (5 mL) | Live yeast culture? (50 mL) | Sugar added (mL) | Ethanol added (mL) |
1 – control | YES | NO | 0 | 0 |
2 – control | YES | NO | 0 | 0 |
3 - control | YES | NO | 0 | 0 |
4 | YES | YES | 0 | 0 |
5 | YES | YES | 0.25 | 0 |
6 | YES | YES | 0.5 | 0 |
7 | YES | YES | 0 | 0.25 |
8 | YES | YES | 0.25 | 0.25 |
9 | YES | YES | 0.5 | 0.25 |
10 | YES | YES | 0 | 0.5 |
11 | YES | YES | 0.25 | 0.5 |
12 | YES | YES | 0.5 | 0.5 |
Procedure for measuring absorbance (in absorbance units, or AU)
7. Calibrate the spectrophotometer:
Turn on the spectrophotometer and let it warm up for 15 minutes. You will get erroneous results if you don’t let it warm up first.
Be sure the spectrophotometer is set to read at the wavelength of 550 nm
With no tube in the spectrophotometer and the lid closed, use the left-hand knob to adjust the reading to 0% Transmittance/push zero button to calibrate
Insert a CONTROL tube (making sure it is clear, without bacterial contamination which would make it cloudy), and use the right-hand knob to readjust the spectrophotometer to 100% Transmittance.
When reading the absorbance, be sure to line up the needle on the spec with its reflection.
8. Immediately before reading any tube, vortex the tube so that the spinning column reaches the bottom of the tube for several seconds. This is critical! The yeast cells are heavy and will tend to sink to the bottom of the tube, so you must vortex the tubes to resuspend them: otherwise, your spectrophotometer readings will be erroneously low. If the vortex is not enough to suspend the pellet of yeast cells at the base of the tube, take a piece of Parafilm and cover the top of the tube, then cover this with your thumb and shake the tube vigorously. The pellet should dislodge and the yeast cells should be easily resuspended after doing this. Use a Kimwipe to wipe down the outside of each tube, to remove fingerprints and other smudges that could affect the absorbance reading. (COULD BE A POTENTIAL ERROR)
9. Record the absorbance (in absorbance units, AU) for the tube on your data sheet.
10. Repeat steps 5 and 6 for every tube.
11. Leave the spectrophotometer turned on for the next user.
Figures you should include are:
Average absorbance vs. time for the no ethanol (0 mL) treatment
Average absorbance vs. time for the 0.25 mL ethanol treatment
Average absorbance vs. time for the 0.50 mL ethanol treatment
Sugar added vs. average carrying capacity (K). Use different symbols to denote each of the three alcohol concentrations
A. After a limit, the increasing concentration of sugar decreases the carrying capacity and growth rate. This is because at higher sugar concentrations, the medium becomes hypertonic and the yeast cells loss water towards the medium.With increasing concentration of the ethanol, the carrying capacity and the growth rate decreases. Why does this happen?
B. Is there any interaction between the effects of adding sugar and alcohol on yeast?
C. why do some cultures not reach K?
D. What are the potential sources of error and assumptions made in this experiment?
E. What do these results mean in a more general (non-yeast) context?