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Another poster!

I couldn’t make the Midwest Ecology and Evolution Conference, but I made a poster. It describes preliminary results from an aphid addition/exclusion experiment I conducted in the summer of 2011. Specifically, it examines the question of whether aphid infestation influences the presence of leaf damage by other herbivores.

MEECPosterKMullerFinal.pdf

X-ray Radiation Dose

Hello everyone! This is Sebastian with another update on the x-ray machine. This post will discuss the various methods that can be used to determine the radiation dose of our x-ray machine. Below you will find my report on determining x-ray radiation doses.

Evaluating 3 methods for estimating radiation doses
23 March 2012
Sebastian Di Clemente

Introduction:
The population biology lab is trying to determine the dose of x-ray radiation that the x-ray tube emits per x-ray taken. Calculating the radiation dose is not an easy task because there is no straight forward way to do it. Each method used to determine the x-ray dose presents several differences in measure and calculation. Knowing the radiation dose of the x-rays can be used to determine what dose levels will hinder or harm a seed and what dose levels may even be beneficial to seeds; in short, knowing the radiation dose will allow researchers to quantify the point where seeds are affected by the radiation. With this experiment I will evaluate the sources that give the x-ray radiation dose and analyze the information given by each source.

Objectives:
1. To determine what method gives the most accurate information
2. To determine what method should be consulted to find the most appropriate radiation dose

Methods:
I gathered information based on web searches, contacting professionals, and contacting the x-ray machine manufacturer. I 1.) found a web page that calculates the x-ray radiation dose level and 2.) the manufacture provided the information that they have on dose levels that the Faxitron MX-20 machine produce at various settings. After receiving this information I test the web calculator by inputting the same settings that the manufacture provided and then compared the calculator reading to the value given by the manufacturer. I also further examined the information that the manufacturer provided and determined any differences in information or information format. The use of 3.) a dosimeter would give the most accurate measurement.

Results:
After comparing the web calculator result to the information given by the manufacturer using the same settings and criteria there is a significant difference in the dose level given. The web calculator had a dose level that was greater than the valued indicated by the manufacturer for lower level voltages (less than 20 kV), but the manufacturer indicated a greater dose level at anything above 20kV compared to the web calculator. The professionals offer the solution of a dosimeter. The comparison of the manufacturer data to the web calculator, and the three methods are provided in table below.

Comparison between manufacturer data and web calculator:

View image

The web calculator:

http://www.radprocalculator.com/XRay.aspx

The information given by the manufacturer is given in the following documents:

Dosage MX 20.pdf

mx-20 EXPOSURE DATA.pdf

MX-20 mR Ouput versus time.pdf

The professionals offer the solution of a dosimeter.

Conclusion:
Considering all of the information that I gathered I would trust the manufacture data over the web calculator data. The web calculator is good for fast calculations and changing between what units the dose level will be expressed in. Although, after testing the web calculator and see such a significant difference between it’s calculation and the manufacturer data, I feel that the manufacture would be more likely to have more accurate information.

Since the manufacture data is most reliable it is the clear choice to use. The manufacturer data covers more information, such as time, voltage, as well as unit conversions for other factors. Considering that more information is provided more variations to experiments can be made and the radiation does would still be available after simple unit conversions.

The other option presented by professionals would be to use a dosimeter to directly measure the radiation dose. This option would be the easiest way out of the three options, and would cater more to a researcher’s specific setting. If a dosimeter is available to use I would make this device my choice for determining radiation dose.

Dichanthelium Update!

Hi everyone!

Maria here. Sorry that I have not posted since the end of summer, but please rest assured that I’ve not run away with my Dichanthelium seeds, but have been working on them for the past -what? 6 months? A long and intimate relationship indeed.

Brief summary of what has happened:

I did a pilot germination & growth study using bulk Dichanthelium seeds. The results of germination study is nicely summarized in this poster that I presented at Midwest Ecology and Evolution Conference (MEEC) in Cincinnati 2 weekends ago(?). MEEC was fun and presenting (yapping about) my poster was a lot less nerve-wracking than I had expected:
MWangMEEC2012poster_44_x_36.ppt
Thanks to everyone who helped me in my hectic rush to get the poster done X_X

The seedlings are currently growing in the growth chamber at CBG. (There’s pictures in the poster of seedlings in agar and in plug trays!)

I shall put up some more pictures sometime in the future.
There’s a series of pictures I want to put up showing seeds before and after x-ray and scarification – it’s pretty interesting.

I should also post the R script I used to analyze data and produce the graphs on the flog – unfortunately don’t have the file on this computer.

Right now I’m working on scarifying Dichanthelium seeds for my maternal lines growth and germination experiment (probably should explain in better detail later, likely in another poster).

Other good news you might find interesting:
Thanks to A LOT of help from Stuart and other advisers, I applied and got the Northwestern Academic Year Undergraduate Research Grant for my Dichanthelium project during the school year (maternal line germination/growth experiment), and also very recently, the Garden Club of America Clara Carter Higgins Summer Environmental Study Scholarship =)

If you have any questions about Dichanthelium or anything I talked about, you’re welcome to get in touch. My email is right under the entry title.

X-ray Machine Magnification

Hello Project Echinacea Flog!,
My name is Sebastian Di Clemente I am the Lake Forest College 2012 spring intern class of 2013, and I am quite excited about, this, my first post. I’ve been assigned the project of determining the best settings and magnifications for the new x-ray machine. Below you will find my report about the various magnification levels.

X-ray machine magnification
27 February 2012
Sebastian Di Clemente

Introduction:

The population biology lab is trying to determine the best x-ray magnification to use for scanning Echinacea achenes. The criteria that constitute “best” are image quality and contrast, label legibility, and overall time and efficiency. Each magnification presents different advantages and disadvantages, some more prominent than others. The use of these x-rays can give a more definitive answer of whether an achene has been fertilized compared to achene weight. With this experiment I will evaluate the x-ray machine magnification levels and determine the best choices and ideally isolate one magnification setting that would be best.

Objectives:

1. Obtain the best contrast quality possible for achenes
2. Obtain the best quality setting to read the label on the envelope
3. To determine the best settings and magnifications to use to maximize both label legibility and achene contrast

Methods:

I scanned batches of Echinacea achenes in envelopes under the 10 second and 18 kv setting on the x-ray machine at the varying magnifications (magnifications are 1:1; 1:1.5; 1:2; 1:3; 1:4; 1:5) and window level settings. After taking a number of images at each magnification and assigning the prescribed window level settings (see X-Ray Machine Protocol for Echinacea) I compared images side by side. I then documented similarities and differences, and pros and cons of each image on their own and in relation to the other images taken. Based on the resulting images and my notes, I determined what each magnification might be useful for. Finally, I choose two magnifications out of the six that I thought would be most useful, and then weighed the pros and cons of each one more heavily and made my final choice as to which magnification would probably be best.

Results:

1:1 Magnification

1 To 1 Mag.jpg

At the 1:1 magnification the labels are hardly visible. The zooming in on this image would not do that much good because the image will become more pixilated. It is quite difficult to distinguish the achenes that are hollow and have not been germinated. Also, it is not possible to tell where the envelopes end or begin. The only real benefits of this setting are that four envelops can be scanned at a time and the achenes that have an embryo can be fairly easily counted.

1:1.5 Magnification

1To 1_15 Mag.jpg

A magnification of 1:1.5 clearly does not show the greatest image. Although three envelopes can be captured in the image the labels are rather difficult to read and part of the third envelope gets cut off. The orientation of the envelopes is also a bit confusing and more laborious to set up. Positives of the image are that a large sample of achenes can be processed at a time. Another benefit is that after zooming in on the picture the achenes are easy to count and the visibility of germinated and non germinated achenes is fairly clear.

1:2 Magnification

1 To 2 Mag.jpg

The first benefit the 1:2 magnification has is that two envelopes can be scanned at a time. This benefit can double the speed of the scanning process. The extra space around the two envelopes can be use to include any smaller envelopes that may come inside the main envelope. The labels in this setting are still readable and the achenes show up nicely. The image needs to be zoomed in upon to provide a more accurate count of the achenes and to tell which have been germinated and which have not. If time is not of the essence, one of the magnification settings soon to follow would be recommended.

1:3 Magnification

Best Compromise 1To 3 Mag.jpg

The magnification setting of 1:3 is a good compromise between the previous settings and the settings to soon be discussed. This setting provides an image that encompasses a full envelope and leaves some room to spare. The extra room can be used for adding any small envelopes used to set aside certain achenes that may come inside the main envelope. The label in this image is fairly legible and every achene can be counted. It is also possible to determine which achenes have an embryo or are lacking an embryo. Furthermore, if the image is zoomed in upon it is possible to see any damage or defects of the achenes. The only issue with this magnification setting is that only one envelope can be scanned at a time, which makes the overall scanning process proceed at a slower tempo.

1:4 Magnification

1 To 4 Mag T-3 Best.jpg

A 1:4 magnification setting provides a fine image that shows both the label and the achenes clearly. From this magnification it is easy to count achenes, see any damage or defects of achenes, and tell whether achenes are hollow or have an embryo. Drawbacks to this setting are that the entirety of the envelope is not captured in the image, which leaves achenes not visible at the bottom or top of envelop that is cut off. Another obvious set back is that it is only possible to view one envelope at a time. This setting would be recommended to use if a close examination of the achenes is need, especially when trying to examine a greater number of achenes at a time.

1:5 Magnification

1 To 5 Mag.jpg

At a 1:5 magnification the clearest results are returned. Each achene can easily be counted, identified as hollow or full, and the label is clearly legible. This magnification is the highest magnification possible on this x-ray machine and is therefore the high-end extreme. The negative aspects of this magnification are that it is not possible to capture the entire envelope in the image. Unless all of the achenes are pushed towards the label there is no way of telling how many achenes may not be accounted for. As a result of not being able to fit one full envelop in the image it is not a far stretch of the mind to understand that capturing two envelopes at this magnification setting is out of the question and that only one envelope (or part of one). At this magnification, it would only be recommend to be used to examine certain achenes in order to inspect damage, shape, or any other anomaly that is being investigated.

Conclusion:

Considering all of the magnification settings, the top two would have to be 1:2 and 1:3. These levels have the most benefits out of all of the other settings without all of the negatives of the other settings. These two options are thus recommend for use. The question that presents itself is a matter of time and efficiency, and what setting is best to use. At the 1:2 setting, does the time saved by scanning two envelopes at a time out weigh the time it would take a person to zoom in on each envelope and count the achenes and determine which are germinated and which are not? At a 1:3 magnification, does the time to scan one envelope at a time and continually switch out samples negate the time it takes for a person to count the germinated and not germinated seeds without zooming in?

After carefully considering the question of time and efficiency I conclude that the 1:2 magnification setting is indeed the best choice and the 1:3 setting the second best choice. The time it takes zoom in on one envelope to count the achenes and determine their germination states and then zoom out and zoom in to do the process over is shorter that the time it takes to scan one envelope at a time and be easily to count the achenes and determine the germination states without needing to zoom in. To zoom in and out and back in takes far less time than completely going through the image scanning process for individual envelopes. The time it takes for the media plate to go through the CR reader is what takes the longest and makes the 1:3 magnification the second best choice.

All accounted for, the best magnification setting to use is 1:2 for time and efficiency sake. If time is not of the essence, then the 1:3 magnification setting would be the best option. The final ranking of all of the magnification settings would be: A.) 1:2 B.) 1:3 C.) 1:4 D.) 1:5 E.) 1:1.5 and F.) 1:1 respectively. This ranking and the best option may very based on the experiment being run, sample size, and what the object of inquiry is. For a general scanning to most efficiently count and determine germination states this ranking holds. If a different experiment is being conducted and or a different sample size or object of inquiry is at hand then the best setting to use should be determined as needed based on the pros and cons as listed in the previous pages.

Scanning distance quality experiment

Hello Project Echinacea Flog!,
I’m glad to be posting my first post! I’m Ricardo Rivera, and I started working for the lab in December and it’s good to be back after the winter break. Seed cleaning for the 2011 harvest is close to being done and scanning achenes for counting is the next step. Karen Taira and I were given the task to try out a new scanning surface and provide feedback about how it could be improved. I have attached the report that Karen, Stuart and I completed.

Report:
Revised Scanning Glass experiment.pdf

Appendix
Control Image:
rkExpTrCont001.jpg
3mm Glass to glass distance:
rkExpTr5001.jpg
5mm Glass to glass distance:
rkExpTr1001.jpg
7mm Glass to glass distance:
rkExpTr2001.jpg
9mm Glass to glass distance:
rkExpTr6001.jpg
13mm Glass to glass distance:
rkExpTr3001.jpg

More Microscopic Images

In the lab, we have found more insects, a spider, and a lot of web in the Echinacea heads we have been cleaning. The insects include another lacewing fly and two beetles that I cannot identify. I also found a hard shell that looks like a Syrphid fly pupal case. I have the web and the egg sacs clustered because of the amount that we tend to find in the lab.

Unidentified Beetle No. 1:
Capture_00010.JPG
Capture_00011.JPG
This beetle is black with two longitudinal yellow stripes down its dorsal side. It has wings and extended back legs for jumping. The mouth part is a golden color, similar to its legs. It also has reddish colored eyes. The beetle’s wings extend pass its abdomen slightly. The beetle also has very small antennae.

Unidentified Beetle No. 2:
Capture_00012.JPG
Capture_00013.JPG
This beetle’s body has been flattened in the bag or during cleaning. It is brown with lighter brown wings. The wings do not expand past its thorax. The beetle’s legs are short. The thorax and the abdomen form a pentagonal shape. The eyes are a dark brown color.

Lacewing Fly:
Capture_00018.JPG
This lacewing fly has different characteristics in the abdomen than the previous one I posted. I suspect that the insects are different genders, based on the different abdomen shapes, but I was unable to find anything on sexing lacewing flies.

Spider:
Capture_00016.JPG
Capture_00015.JPG
I suspect this spider to be a type of jumping spider due to the body and leg shapes and the fact that it has eight eyes. The four smaller eyes can be seen on the back of the head and this gives the spider more accurate vision and a wider range of sight. The spider’s head has a square shape with four eyes in the front and two eyes on each side. They are very hard to see, but there is a slight reflection of light where the other four eyes are located.

Syrphid Fly Pupa Case:
Capture_00017.JPG
This is a hard, transparent shell of either a larva or a maggot that I could not identify. Stuart suspects that it is from a Syrphid fly pupa. The piece sitting next to it was broken off when I was moving the specimen with the forceps.

Spider Web Cluster:
Capture_00014.JPG
This is a cluster of web and egg sacs that we have found in the Echinacea plant material. We tend to find a lot of web and egg sacs when cleaning Echinacea heads.

2012 Planned Common Garden Measuring Protocol

Here is the protocol that we plan to use for measuring in 2012:
2012.measureFieldProtocolPlan.htm

2011 Common Garden Measuring Protocol

Here’s a link to the protocol that we used for measuring CG1 in 2011:
2011.measureFieldProtocolReal.htm

In 2012 we plan to measure in “review mode” (as we did for CG2 in 2011) — all location records will be on the Visors with Status=”Staple” or “Skip” populated. We should not spend as much time searching for plants that have not been present for 3 or more years.This should speed up measuring. I’ll post the planned 2012 protocol next.

Heads in CG1

Now that we’ve inventoried all the CG1 heads, I checked to see just how many we have. There were about 3009 twist-ties put out, and 119 heads were duds or missing, so our (estimated) total number of good heads is about 2890.

CG2 had something like 140 heads, but we haven’t inventoried those yet.

Aphids attack inbred plants

In a paper just published in PLoS ONE, Echinacea Project researchers show how habitat fragmentation may make plants more susceptible to aphid attacks. Aphid abundance early in the season is higher on inbred and outcrossed Echinacea angustifolia plants compared to regular plants. Elemental stoichiometry plays a role in this plant-herbivore interaction, but other genetically-based plant traits must also attract or encourage aphids.

Ridley CE, Hangelbroek HH, Wagenius S, Stanton-Geddes J, Shaw RG, 2011 The effect of plant inbreeding and stoichiometry on interactions with herbivores in nature: Echinacea angustifolia and its specialist aphid. PLoS ONE 6(9): e24762. Available online at http://dx.plos.org/10.1371/journal.pone.0024762.