Yaamini’s Notebook: Gigas Spawn

Spoiler: We have baby oysters!

I successfully spawned my Pacific oysters this weekend! A huge shoutout to everyone who helped me over the past two days: Rhonda (#TheRealMVP), Steven, Kelsey, Ashley, Megan and Laura.

The relevant data and calculations from my spawn can be found here.

Saturday, July 29

Step 1: Shuck and sex all oysters

The first thing we did was open up all of the oysters and put them into individual paper boats. This was to keep each oyster separate and avoid contamination. We kept all oysters that looked ripe. Anything that looked a little questionable was kept just in case.

img_3115

img_4968

Figures 1-2. Rhonda, Ashley and Megan shucking open oysters.

img_3036

img_3050

img_3086

img_3089

Figures 3-7. Examples of ripe oysters.

Using a capillary tube, I took a bit of gonad sample and examined it under the microscope.

img_4969

Figure 8. Kelsey adding a capillary tube to a shucked oyster.

img_3104

Figure 9. Me sexing an oyster. #ActionShot

It was easy to identify which ones were male and female! Males had active sperm, meaning that they were small and swimming around. Eggs do not have a round shape before being in water, but they look like small seeds.

img_3037

Figure 10. Sperm under 10x magnification.

img_3097

Figure 11. Eggs under 10x magnification.

Step 2: Create cross matrix

Once we sexed all the oysters, we had to figure out how many crosses we could do. We only had 14 male oysters from all OA tanks, and 2 from the heat shock tanks. To fit the number of buckets we had, we decided to collapse all of the females into pools by treatment, so there would be three egg pools total: one low pH female pool, one ambient pH female pool, and one heat shock female pool. We could then cross each of the OA males with the low and ambient pools, giving us 28 crosses. Replicating these crosses in two buckets would give 56 buckets. Doing the same for the heat shock oysters, we had two crosses with two replicates, so four additional buckets.

Step 3: Strip all gonads

Once we knew what our crosses were, we took each oyster and stripped the gonad. Using a sharp pointy blade, we scored the back and front of the gonad. Then, we scooped the gonad into a pre-labelled tripour. For the females, we stripped 1 gram of gonad per oyster to create our pools. Two of the males ended up not being ripe, so we threw those out and did 52 total crosses instead.

img_3129

img_3133

Figures 12-13. Scoring and scooping the gonad into a tripour.

Step 4: Prepare eggs and sperm for fertilization

  • Screen sperm on an 80 micron screen and catch on a 20 micron
  • Screen eggs on 80 micron screen and catch on 20 micron
  • Combine all relevant eggs for each pool
  • Hydrate eggs for 45 minutes
  • Count eggs in each pool
  • Calculate the number of eggs needed to fertilize each cross

Step 5: Fertilize!

  • Add calculated amount of eggs to a tripour for each cross
  • Add sperm
  • Let eggs fertilize for 20 minutes
  • Check for polar bodies to confirm fertilization

img_8097

Figure 14. Polar body on one egg.

Step 6: Distribute fertilized eggs to 5 gallon buckets

  • Buckets should hold at 23 ºC
  • Water bath should hover around 23-24 ºC

img_8099

img_8101

Figures 15-16. Static system pictures post-fertilization.

Sunday, July 30

Step 1: Check developmental stage

When we first got to the hatchery, the larvae were trocophores. This could be because we only fertilized around 6 p.m., and they require about 18 hours to become D-hinge. We only want to handle D-hinge since they hold on a 48 micron screen, and we would be able to account for slower-developing larvae.

screen shot 2017-07-30 at 10 54 01 pm

Figure 17. Trocophore larvae around 9 a.m.

img_8115

screen shot 2017-07-30 at 10 54 35 pm

Figures 18-19. D-hinge larvae around 11:30 a.m.

Step 2: Screen D-hinge

While screening, we pooled replicates together to reduce the number of counts we had to do.

img_4980

Figure 20. Kelsey screening larvae!

Step 3: Count D-hinge

img_4985

img_4989

Figures 21-22. Ashley dispensing larvae to a Sedgewick Rafter slide, and Laura counting larvae.

Step 4: Redistribute D-hinge to static system

  • Sum total D-hinge per treatment pool
  • Calculate amount of D-hinge to put in each bucket with a stocking density of 4 larvae/mL
  • Put larvae in static system buckets
    • 8 totes, 3 buckets each
    • One tote had a crack, so I had to split the buckets into two separate smaller black totes
  • Fed 60 mL of C.iso and 609 to each bucket

Other notes

While opening the gonad of two female oysters, I found some weird red polychaete thing. I fixed these in 80% ethanol and sent these pictures to Chelsea Wood in case she wanted them!

img_8087

img_8091

Figures 23-24. Weird polychaete things found in oyster gonads.

from yaaminiv.github.io http://ift.tt/2vdusOB
via IFTTT

Advertisements

Yaamini’s Notebook: Manchester Conditioning Update11

Yaamini’s Notebook: Manchester Conditioning Update 10

It’s getting ugly

I had 16 oysters die today from various treatments. Based on Steven’s suggestion on Monday, I moved the oyster bags to individual 5 gallon buckets on Laura’s larval heated line, around 18 ºC. When I opened oysters that were dead, they all looked really ripe, and there were no signs of any disease. My guess is there’s something in the combination of the kiddie pool and high temperature that’s getting to them.

Table 1. Revised oyster counts in each tank, as of July 25.

Tag Label A B Total
1 3 7 10
2 5 8 13
3 2 6 8
4 2 7 9
5 6 8 14
6 4 8 12
Heat Shock 3 4 7
Full Amb 0 6 6
Spare 1 3 4
Total 26 57 83

I cut open the ones that were dead and with the exception of two, preserved them for future testing. Three oysters were stored in falcon tubes with ethanol, three in the freezer and a jar with about six oysters was put in the fridge. Not entirely sure what to do with them yet, but at least I have them. The ones that were died were quite ripe and did not look unhealthy.

img_8043

img_8044

img_8054

img_8056

Figures 1-4. Examples of oysters that died.

Oysters in Figures 1-4 were also sexed. All were male.

img_8045-1

img_8046-1

img_8049-1

img_8050-1

Figures 5-8. Microscope images of male gametes.

Other things I did today:

  • Turned off immersion heaters
  • Cleaned algae header and filled with 1.6 L Reed’s paste
  • Removed lines from oyster tanks and bleached algal line
  • Counted about 30 2 gallon buckets that can be used for fertilization
  • Set up buckets for each bag of oysters with 26 L/hr drippers and airstones

img_8055

Figure 9. New set-up.

  • Cleaned gigas and counted mortalities
  • Tried measuring pH of kiddie pool water. Both durafets read different pH values for Pool B (farthest from wall).

img_8053

Figure 10. Durafet monitor readings for Pool B.

  • Put the Heat Shock B oyster we thought had died back into a different bucket since it’s shell was completely closed as we were about to leave.
  • Pumped T.iso in for oysters to feed instead of paste, dosing pump at 50%

Main changes:

  • Each oyster bag has it’s own 5 gallon bucket, increasing flow and reducing density
  • Temperature is now around 18ºC instead of 23ºC. I talked to Rhonda and she’s a bit concerned that the oysters may start to reabsorb their gametes. She once had to drop broodstock to 15ºC two days before a spawn and it was fine. Maybe this will also be okay? Can they really reabsorb that quickly?
  • Oysters are being fed live algae

I will be back Thursday to check on oysters and continue preparing for spawn. I’m really hoping that no more die — I think we’ve eliminated all possible stresses! All I need is for them to be alive until I spawn them.

from yaaminiv.github.io http://ift.tt/2tBz0KV
via IFTTT

Yaamini’s Notebook: Manchester Conditioning Update 9

The mortalities continue

The past few days I’ve seen a string of mortalities, primiarly in conditioning Tank A.

Thursday, July 20

Grace vacuumed the oysters and checked for mortalities while she and Laura were out there. She found three dead oysters: 1 from Tank 1B, 1 from Tank 1A and 1 from Tank 5A. Tank 5A had been dead for a few days, while Tank 1B and 1A were freshly dead.

img_3931

img_3932

img_3933

Figures 1-3. Dead oysters.

Saturday, July 22

Laura cancelled at the last-minute on Saturday, so I took her car and went to Manchester. When I got there, all of her larval buckets were brimming, about to overflow. I replaced the banjos then cleaned the ones I took out. I also checked the heater setpoints.

img_8010

img_8011

Figures 4-5. Heater setpoints upon arrival.

I then started on cleaning my oysters. I immediately noticed that the oyster bags themselves were collecting a lot of fecal matter and algae. Most of my time vacuuming was spent vacuuming the bags. Next year, it may be better not to use these bags and opt for something like a tray that can be removed and cleaned. There were three dead oysters: 1 from Full Amb B and 2 from Tank 3A. When I looked at their gonads, they were milky. Even though my oysters have been consistently dying, they’re also consistently ripe. I need to start sexing them soon and checking for active sperm.

fullsizerender

img_8008

img_8017

Figures 6-8. Gonad development from dead oysters.

Because of the mortalities, I reduced the right heater setpoint.

img_8012

Figure 9. New heater setpoint.

I continued my cleaning kick and rinsed Laura’s downwellers with freshwater. I then fed her algae tanks a mix of C.iso and Chagra and checked that the dripper was working. I then added 1.6 L of Reed’s paste to my algae header tank and turned off the dosing pump so I could clean the heating tank.

When I opened the algae heating tank, it looked and smelled like a swamp monster graveyard. The entire tank was filled with dense clumps and string of algae. I think algae had been growing (and dying) in the heating tank before being fed to the oysters. My guess is that this was causing some of the oyster deaths.

img_8016

Figure 10. An example of what was growing inside the heating tank.

As I was cleaning the heating tank, I also wanted to flush algae from the water line. When I increased flow from my heated line, I noticed there was no water. I called Laura and saw that her outside tanks were also getting no water. The water shut off at some point while I was eating lunch, so it wasn’t off for more than an hour. Luckily, Rick stopped by the hatchery at that time. He discovered that the float valve in our seawater reservoir tank in the warehouse had been jammed in a way that prevented water from flowing. He was able unjam it and get water to flow again.

Another thing I noticed on Friday was that the two tanks had a 1.5ºC-2ºC difference in temperature. After cleaning the heating tank and pipes feeding water to the kiddie pools, I visually adjusted flow so they looked equal in both tanks. I checked the AVTECH monitor and saw that temperature in both pools were within 1ºC. I had to catch a ferry and didn’t have time to measure flows. I set the dosing pump to 60% and ran out the door.

Sunday, July 23

Laura went out to Manchester so she took a look at my oysters. The first thing she found was a high number of mortalities: 2 from Tank 3A, 2 from Full Amb A, 1 from Tank 5A, 4 from Tank 4A, and 1 from Heat Shock B. She also saw that the pools were extremely dark when she got there and the food was completely dark. This means that in 24 hours, the oysters were fed 1.6 L of Reed’s paste. It’s possible that they were suffocated by their own lunch.

52253308340__3cfb02ab-0675-44e8-9e5e-e66669f7945a

52253309681__ce12a3f1-c9a5-47ce-b874-6060e2bbc379

52253312011__f30a3470-021b-4375-b63b-44d8658dfcef

52253312803__4c99c913-12c5-4ad1-bca8-cdb212b93570

52253314790__d2f9e81d-907d-4f2f-b70d-a72c2fdf0c21

Figures 11-15. Dead oysters.

I also had her open the oysters that were recently dead.

img_2311

img_2312

img_2313

img_2314

img_2315

Figures 16-20. Gonads of recently dead oysters. All are milky and ripe.

The algae heating tank was not dirty, which was good. Because the pools were slimy and filthy, Laura cleaned them. However, this meant that she moved the oysters out of the water. I’d been avoiding this because I was told they would spawn out. Laura, however, did not know this. She adjusted flow to 2 L/min into each kiddie pool and set the dosing rate to 40 after adding 750 mL of food to the algae header. Before she left, she checked to ensure the oysters had not spawned out.

Monday, July 24

No mortalities today! I took care of a couple of others things while I was out after cleaning the kiddie pools and heating tank. I counted about 60-70 tripours and obtained 8 totes that fit 3 buckets each. I need one more tote to fit 25 buckets total.

Table 1. Revised oyster counts in each tank.

Tag Label A B Total
1 6 7 14
2 8 8 16
3 2 6 8
4 2 7 9
5 7 8 15
6 5 8 13
Heat Shock 5 5 10
Full Amb 2 7 9
Spare 2 3 5
Total 39 60 99

from yaaminiv.github.io http://ift.tt/2uRDkJE
via IFTTT

Laura’s Notebook: SRM Dilution Curve Sample Prep

Prepping dilution curve samples

After we run all our samples Yaamini & I are going to run 10 samples with mixtures of geoduck/oyster protines. We will prepare them at different, known preportions of G:O, and see how the peptides we each targeted become more/less prevalent. This is good practice to prove that we are measuring what we say we are.

Yaamini did a great job calculating/writing up the dilution calculations (after a couple iterations, see here and here

As Yaamini did, I pooled 5ul of 5 randomly selected samples for a total of 25ul of pooled sample – I selected samples that had the full 2ug/ul (as opposed to those that had low concentration), pipetted them into a centrifuge tube, vortexed, then spun down gently:

  • 120
  • 47
  • 79
  • 60
  • 9

Then, I got Yaamini’s dilution curve samples, that already have PRTC & ACN+FA, out of the freezer, and pipetted the designated vol of my pooled geoduck sample into each tube:

image

Then I vortexed each, spun down gently, labeled autsampler vials, and transferred the dilutions into the vials. I put them in the -20 freezer until we are ready to use them.

from LabNotebook http://ift.tt/2v19XVQ
via IFTTT

Laura’s Notebook: Remaining SRM Timeline

How many samples can I run?

@ 8:30am on Monday 7/24 I got my samples started again. I need to figure out how many more samples I can run within the given timeline. Here are the considerations:

  • Running samples in batches of (5 samples) + (1 QC) + (1 blank) = 500 minutes total, so that’s 100 minutes / sample.
  • We have until 10am on Friday 7/28
  • Need 40 hrs for the dilution curve run
  • So, need to be done with my samples by Wednesday 7/26 @ 6:00pm
  • Time between this morning @ 8:30am when I re-started my samples & 7/26 @ 6pm = 57.5 hrs = 3450 minutes / 100 minutes/sample = 34.5 samples.
  • I have 25 samples left to run, plus 2 blanks (Gblank & OBlank) which I could run twice.
  • Should be done with my samples on Wednesday @ 5:30am, this includes 1 run of each blank.

Thoughts on whether or not to re-make samples

Up to this point I have 20 samples where a handful of peptides don’t show up from both PRTC and my samples. In PRTC there are 4/9 poor quality peptides, and in my samples 3/39 poor quality transitions. In an ideal world I would remake these ~20 samples, run the new batch twice while being careful with freeze/thaw and time out of the freezer. However, I don’t have time for 2 runs of remade samples. I could remake, then do 1 run of each in the hopes of capturing data on those 3 transitions. However, I think it’s best to have replicates of the 36 good quality transitions in my samples. Also, the 3 poor quality transitions were not in the sample proteins, so I can likely draw conclusions about protein quantification from the other 2 transitions. The differing rates of peptide degradation between samples does make me a little concerned; I’m wondering how folks take this into consideration.

Samples left to run:
#### Plate 2 – 23 + 2 blanks | | 1 | 2 | 3 | 4 | 5 | 6 | 7 | 8 | |—|——–|——–|——|——|——|——–|——|——| | A | | | | | | | | | | B | G041 | G066 | G105 | G032 | G129 | G054 | G081 | G003 | | C | G074 | G014 | G049 | G053 | G104 | G055 | G042 | G064 | | D | G073 | G057 | G007 | G070 | G001 | G071-B | G062 | | | E | GBlank | OBlank | | | | | | | | F | | | | | | | | |

#### Plate 1 – run 1 – 1 sample I didn’t re-run | | 1 | 2 | 3 | 4 | 5 | 6 | 7 | 8 | |—|——|——-|——|——|——|——–|——|——| | A | | | | | | | | | | B | | | | | | | | | | C | | | | | | | | | | D | | | | G128 | | | | | | E | | | | | | | | | | F | | | G122 | | | | | |

NOTE:

  • The following samples were put into the autosampler tray @ the following dates/times:
    • 7/23 @ ~8pm: G041, G066, G105, G032, G129, G054, G081, G003, G074, G014, G049, G064, G073, G007, G001, G071-B, G062.
    • 7/24 @ 2:25pm: G122
    • 7/24 @ Xpm: TBD
    • 7/25 @ Xpm: TBD

from LabNotebook http://ift.tt/2vCE5UJ
via IFTTT

Laura’s Notebook: Mass Spec, good things to know

Pro Tips for using UWPR mass spec

  • On the nanoAquity UPLC Console keep an eye on the Binary Solvent Manager screen to monitor pressure. Right click over the plot area, click Plot Properties, and change the time frame to 10 hrs.
  • If you miss-assign a vial location, or remove a vial too early (like I did), the mass spec will sense this and display an error “missing/wrong plate or vial”. It will stop running. The AutoSampler program will need to be reset, and sometimes also need to hit the manual reset button on the machine. Use the same process as when a program is not responding:
  • If program is not responding, wait until the current sequnce is done, then it may start responding. If still not responding, close the program and re-open. do the following:
    • On Thermo XCaliber go to Status tab on the left side of the screen
    • Check that under Waters nanoACQUITY and TSQ Vantage they both read “ready to download” – if so, you can start your run.
    • If an error, close all programs, reboot PC.
    • Open these 3 windows: Thermo Sequence Setup, Xcaliber, NanoACQUITY UPLC Console, Thermo TSQ Tune Master. It may automatically connect. If not:
    • Hold RESET tiny black push button down for 3 seconds. This should connect the software to Vantage.
    • Before running sequences, on Xcaliber, select Actions -> Automatic Devices On
    • Select & add desired sequence rows
    • Push green “play” button – should work out.
  • If you try to open a raw file in Skyline and it says “permissions denied” or something like that, try closing Skyline and re-opening it.
  • In Thermo Xcaliber Sequence Setup, be careful when modifying the sequence table:
    • If you’ve already added a row to the Acquisition Queue, but you want to change something in that row, DO NOT simply edit then re-add it. Instead:
    • First, delete the rows in the Acquisition Queue that you no longer want by: clicking check box, then hitting the Delete button on a Windows keyboard, or FN+Delete on a mac (if using Team Viewer)
    • Second, start a new row in the sequence table, complete all cells, then add that to the queue.
    • Do not edit then re-add any rows that have already been added to the queue.

Making a method

  • It’s best to work with someone who has used your machince before, get a method from him/her, and tailor it to your needs. Prisca, or someone from the McCoss lab have helped Emma in the past.

Mass Spec Setup tutorial

  • Things that are sitting out in the UWPR mass spec room are things that you can use
  • First thing to make is the pre-column for the trap, we used 4.5cm, with the frit ~3mm. Trap is wider diameter 100um, and different material. Sample first goes on to the pre-column, junk is washed away within the pre-column. When installing: frit points towards the mass spec.
  • Then, go to the nanoQCQUITY; start testing your columns to make sure they can handle the pressure during your sample runs
    • Click on 0.000 uL/min, select “Trapping”
    • Solvent A: 0.3 ul/min, 5% Solvent A
    • Confirm it’s still trapping
    • Watch pressure change on top plot; make sure it doesn’t go too high
    • Change the flow rate on A1 to 0.5 ul/min, after it levels off record pressure
  • Attach analytical column.
    • look at it in the light, make sure there are no bubbles
    • Attach
    • Change solvent B to 5%, analytical, and @ 0.2ul.
    • Keep an eye on the tip of the column; once a droplet begins to form, wait 10 mins. If pressure looks good, then… TB continued…

from LabNotebook http://ift.tt/2vBJ4Vr
via IFTTT