Melanoma epidemiology, etiopathogenesis and prevention - Professor Torello L...
2009 NSA
1. L.M. CROSSON*, C.S. FRIEDMAN. School of Aquatic and Fishery Sciences, University of Washington, Seattle, WA 98195. J.F. MORADO. National Oceanic & Atmospheric Administration, AFSC, 7600 Sand Point Way NE, Seattle, WA 98115.
2. BCS is a fatal disease caused by an undescribed parasitic dinoflagellate of the genus Hematodinium Hematodinium proliferates in hemolymph – alters hemolymph chemistry metabolic exhaustion death Infects numerous species of decapods & method of infection is unknown Left : Heavily infected Chionoecetes bairdi Right : Hematodinium infected (top) versus healthy (bottom) C. bairdi
16. Design primers Conventional PCR Insert amplicon into plasmid Clone multiple copies of plasmid Purify plasmid Quantify plasmid copy number Create dilution set Create standard curve with QPCR Graphic courtesy of Nate Wight
17. 30M 3M 300K 30K 3K 300 30 3 Comparison of cPCR to QPCR. Conventional PCR can reliably detect 300 or more copies, while QPCR can detect as low as 3 copies indicating that QPCR is 100 times more sensitive than cPCR cPCR QPCR
18. Dissociation curve analysis with a single peak illustrating the presence of a single DNA fragment amplified by the QPCR test
21. Port Camden Holkham Bay/ Stephens Passage Glacier Bay Icy Strait Douglas Island 0% Port Camden 8% Holkham Bay 10% Thomas Bay 0% Glacier Bay & Icy Strait 10-20% Douglas Island Thomas Bay
22. 2006 Glacier Bay = 0% 2005 Holkham Bay = 8% Stephens Passage Glacier Bay Blood Smears 40% 2% QPCR 64% 12%
BCS is a fatal disease caused by an undescribed parasitic dinoflagellate of the genus hematodinium. The dinoflagellate proliferates in the hemolymph or blood and alters the hemolymph chemistry leading to metabolic exhaustion of the crab and ultimately death. Hematodinium is known to infect over 20 different species of decapods however the method of infection has yet to be determined.
Some commercially important species effected by this disease are snow and tanner crabs, blue crabs, and the norwegian lobster. The map shows worldwide reports of hematodinium related disease. The distribution of this disease is global, having severe impacts in AK, Canada, the eastern US, Europe and even Australia. It is also important to note the majority of new infections have occurred in commercially important decapods in northern temperate zones that are experiencing increased warmer temperatures.
Some signs that are indicative of hematodinium infection are that the animal becomes lethargic with drooping limbs and mouthparts, its exoskeleton will have a cooked appearance as shown by the infected crabs highlighted in yellow, the animals hemolymph will be milky white in color, and the arthrodial membranes will turn from translucent to opaque. While hematodinium is not known to cause harm to humans, it does however give the animals meat a chalky texture and bitter taste deeming it unmarketable.
Prior to 1985 there were 7 decapod species reported to harbor hematodinium infections. Currently the disease has been reported in over 20 species worldwide with some areas in SE alaska, such as lynn canal, show prevalences as high as 95% of the population sampled. Mortalities and fishery impacts associated with hematodinium epidemics and the potential for this pathogen to impact affected commercial decapod abundance and distribution patterns are significant. Economic losses attributed to this parasite in the tanner crab fishery alone are estimated to be at least 3 million dollars.
While epidemics and mortalities of commercial size decapods are significant, evidence suggests that hematodinium associated disease is more prevalent in juvenile decapods than in adults and that a high percentage of small infected crustaceans die before they can recruit into the fishery. The parasite is also more prevalent in female than male crab providing additional potential for population and fishery impacts. For example strong bering sea snow crab cohorts in 2000,2001,2002 did not materialize and recruit into the fishery. A potential cause for these failures is Hematodinium. The highest prevalences of infection are found July through October with peak mortalities occurring in August and September. Cooler winter temperatures are thought to inhibit parasite reproduction.
This is a simplistic diagram of the life cycle of a parasitic dinoflagellate. For most dinoflagellates, the dinospore is the infectious stage and once entering a host will begin to grow as a trophont, then become a mobile plasmodia, and reproduce to form new spores.
Here are some typical parasite morphologies. Note the elongated motile plasmodia stage is very easy to discriminate. However, the trophont stage of the parasite looks very similar to the actual hemocytes of the host which can make diagnosis of this disease by microscopy alone particularly difficult and can lead to underestimation of disease prevalence.
To date only 2 species of hematodinium have been fully described from life history stages encountered in infected crabs. Others have not because few differentiating morphological characteristics exist and not all parasitic forms are encountered in infected hosts. Hematodinium from Tanner crab may be a new species however without additional characterization of the established and novel strains, the number of species and the extent of host specificity remains unknown.
Disease transmission is thought to occur during the post-molt period and may be enhanced by cannibalism or mating behavior. As I mentioned earlier for many parasitic dinoflagellates the dinospore is the infectious stage, whether this is true for hematodinium awaits further examination. We also do not know if prey species or seawater may possibly be serving as parasite vectors or reservoirs.
So far, in vitro transmission of the disease has not been successful due to loss of infectivity and only partial life histories have been described from infected tissues. In order to resolve the mode of transmission external life history stages require further characterization.
The traditional technique used for pathogen detection is histology. Histology allows you to detect the pathogen and indicate infection status, it is semi quantitative and can be used for downstream analysis such as ISH however the processes is very expensive, time consuming and takes a well trained eye. It also cannot be used to look for pathogen vectors. A molecular techniques that is more sensitive and allows for higher throughput is cPCR but with cPCR you are limited to only presence-absence data. It is not quantitative.
The goal of my project is to develop a molecular tool with high sensitivity and specificity to accurately quantify parasite loads. Being able to quantify parasite loads allows for many new questions to be addressed such as what is the tolerance level of infection before an animal becomes symptomatic? At what infection level is the parasite fatal to its host? Is there a temperature or depth refuge for the host? Do seawater or plankton act as reservoirs for the parasite? Theses are all important questions that we can address using QPCR to help track the proliferation of hematodinium and also to detect very low levels of infection to avoid underestimation of disease prevalence.
QPCR enables the user to quantify loads in a reproducible and high throughput manner. The Taqman probe chemistry employed detects and measures fluorescence as PCR product is produced with each cycle of amplification unlike endpoint detection via cPCR. The probe requires specific hybridization therefore the target sequence must be present to generate fluorescence.
I designed my QPCR assay by first aligning all known 18S rDNA sequences of Hematodinium and related genera using clustalW. I selected sequence areas unique to only hematodinium where I designed primer and probe combinations using Primer3 software. I was then able to develop a hematodinium plasmid standard containing the amplified segment of the parasite genome amplified by my primers. After quantifying the plasmid copy number, a dilution set of known copy numbers was prepared to create a standard curve.
Here is a nice schematic of the steps: I designed my primers, ran a cPCR, took the PCR product or amplicon, inserted it into a plasmid, cloned the plasmid, purified it, quantified it, created a dilution set of known copy numbers, and generated a standard curve with QPCR which I can now use to determine copy numbers of hematodinium DNA in my preserved blood samples.
In Oct of 2006, I was fortunate enough to join ADF&G for their Tanner crab survey where I sampled ~ 60 tanner crab from each location to provide 95% confidence of detecting infections with a prevalence of >5%. Hemolymph was extracted from the arthrodial membrane using a sterile syringe and preserved in ethanol. For every crab sampled gross characteristics were recorded and hemolymph smears were taken for microscopy which will be used as a gold standard against our QPCR assay. Seawater was also sampled, filtered, and preserved from each location to look for parasite vectors.
The prevalences of crabs with visible signs of infection ranged from 0% in Port Camden to ~8% in Holkham Bay and ~10% in crabs from Thomas Bay. These prevalences are similar to those observed on previous cruises with nearly no Hematodinium observed in crabs from Glacier Bay and Icy Strait and ~10-20% in those collected near Douglas Island.
A lot of difference in the zero ……..realtive concordinance in a log linear relationship X blood smear intensity of hemat Y qpcr copy number
In the process of assessing the best way to coordinate data taking into consideration the polymorphic nature of parasite Validating diagnostic and analysitcal sensitivity and specificity.
