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The Use of Ultrasonic Waves as an AlternativeMethod in Mitigating Algal Blooms
By
Madrid, Ludhovik Luiz B.
Medrana, Micholo Lanz B.Morales, Justin Marius D.
Submitted to the Faculty of thePhilippine Science High School – Main Campus
in partial fulfillment of the requirements for
Science and Technology Research 1
March 2011
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ABSTRACT
One type of Harmful algal bloom (HAB) may cause the discoloration of seawater
caused by a dense population of dinoflagellates. However, not all types of HABs can cause
water discoloration. HABs have been recurring in Philippine waters since 1988 and are
notable for their disruption to the marine ecosystem and their negative health and economic
effects. The aim of this project is to determine the effects of time exposure of ultrasound
waves on Pyrodinium bahamense var. compressum to know whether these variables would
lead to inhibition of growth or complete elimination of the organisms.
From an initial culture of the dinoflagellate P. bahamense, 24 Erlenmeyer flasks
containing a 100 mL culture solution will be prepared and divided into 12 separate
experiment groups of 2 flasks each. Each experiment group will test the effect of a same
frequency (1 MHz) on a sample exposed for different time spans. Control samples will
receive no treatment. After each treatment is performed, a cell count will be taken of the
sample using a Sedgewick-Rafter slide and recorded. The results of each experiment group
will be statistically analyzed to determine any significance between the treatments and the
control. This analysis will help determine the optimum exposure time for inhibition of
growth or complete elimination of the organism.
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APPROVAL SHEET
This research work entitled, “The Use of Ultrasonic Waves as an Alternative Method
in Mitigating Algal Blooms” by Madrid, Ludhovik Luiz B., Medrana, Micholo Lanz B., and
Morales, Justin Marius D., presented to the Faculty of the Philippine Science High School –
Main Campus in partial fulfillment of the requirements in Science & Technology Research 1,
is hereby accepted.
____________________________________
Dr. Jessamyn Marie O. Yazon, Ph.D.
Research Adviser
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ACKNOWLEDGMENTS
First, we would like to thank ourselves, for doing our best in working on this
research, and in winning the oral defense in YMSAT. We would like to thank our classmates,
for coming along with us while we “cram” our STR requirements. We would like to thank
our research teacher, Ma’am Yazon, for reviewing on our work, and pointing out mistakes
and improvement on our STR requirements. We would also like to thank some of our
teachers: Ma’am Chupungco, Ma’am Docto, Ma’am Buenafe, and Sir Tan for giving us
advice during the oral defense and Sir Talaue for giving us the research journals that we
cannot access. We would also like to thank the people of MSI (Sir Gar ry, Ate Jenelle, Ma’am
Lita, Dr. Azanza) for helping us in our research, Williard Jose (III-Be), Dr. Jose, and Dr.
Escoto, who helped us find a contact person who has an ultrasound machine, and Mr.
Publico, for letting us borrow his ultrasound cleaner.
Last but not the least; we would like to thank God, for giving us the wisdom, strength,
and inspiration to finish our research, and for giving us hope whenever we had problems in
STR.
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TABLE OF CONTENTS
Page
Approval Sheet i
Acknowledgments ii
Table of Contents iii
List of Tables v
List of Figures vi
I. Introduction
A. Background of the Study 1
B. Statement of the Problem 2
C. Significance of the Study 2
D. Scope and Limitations 3
II. Review of Related Literature
A.
Harmful Algal Bloom (HAB) 5
B. Algal Culture 9
C. Ultrasonic Principles 10
III. Materials and Methods
A. Procurement of Algal Solutions and Other Materials 14
B. Preparation and Sterilization of Culture Flasks 14
C. Preparation of Algal Solutions 15
D. Initial Cell Counting 19
E. Setting up of Ultrasonic Cleaner 20
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F. Exposure of Algae to Ultrasound and Final Cell Counting 21
G. Computation, Graphing, and Tabulation of Collected Data 21
H. Statistical Tests (ANOVA and T-test) 22
IV. Bibliography 23
Appendices
A. Summary of Materials and Methods 26
B. Formulas, Tables, and Graphs needed for Data and Analysis 27
C. Risk Assessment 29
D.
Task List 32
E. Materials Sourcing and Budgeting 34
F. Gantt Chart 36
G. Network Chart 36
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LIST OF TABLES
Table Title Page
5.2.1 Table for Analysis of Variance (ANOVA) 27
5.2.2 Table Comparing Initial and Final Cell Density for each Treatment 27
5.2.3 Table for Correlated T-Test 27
5.2.4 Initial, Final, and Change of Cell Densities of Pyrodinium bahamense var.
compressum cultures in Concentration of Algae vs. Time of Exposure
28
5.3 Risk Assessment Table 29
5.4 Task List of the Methods in the Research Study 32
5.5.1 Table of Materials needed for Experiment and their Costs 34
5.5.2 Table of Transportation and Electricity Consumption 34
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LIST OF FIGURES
Figure Title Page
3.2.1 Erlenmeyer flasks obtained in MSI (left picture), and Erlenmeyer flasks were
cotton seal (right picture)
14
3.2.2 Water filterer connected to a container for filtered seawater (left picture).
Erlenmeyer flask filled with filtered seawater (middle picture). Inside the
autoclave are Erlenmeyer flasks with filtered seawater and seals covered with
aluminum (right picture)
15
3.3.1 Things needed for preparation of algal solutions. From left to right: stock
culture, alcohol lamp, single channel pipette, autoclaved Erlenmeyer flasks
with filtered seawater, and F/2 medium.
16
3.3.2 Aseptic methods for sterilization purposes. Erlenmeyer flask’s mouth was
heated (left), and F/2 container’s mouth was also heated (right)
17
3.3.3 Transferring of F/2 medium from container to Erlenmeyer flask 17
3.3.4 Transferring stock culture to Erlenmeyer flask near the open flame (aseptic
method)
17
3.3.5 All 24 flaks kept near a light source 18
3.4.1 Things needed for cell counting (from left to right): Eppendorf tubes in
orange case, culture flask, and single channel pipette.
19
3.4.2. Researchers working on cell count while looking in the microscope 20
3.5. Ultrasonic Cleaner Set-up 20
5.1. Process Flowchart for The Research Study 26
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5.6 Gantt Chart with Expected Dates of Work 36
5.7 Network Chart of the Research Study 36
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I. INTRODUCTION
A. Background of the Study
A Harmful Algal Blooms (HAB) is a discoloration of seawater caused by a dense
population of a given species of dinoflagellate (Villao, 1988). In some cases, blooms are
accompanied by toxins which, when ingested by surrounding marine life, are capable of
poisoning them or their predators. In the Philippines, especially in the waters of Manila Bay,
HABs are caused by the dinoflagellate Pyrodinium bahamense var. compressum, which have
recurred here since 1988 (Azanza, 1997).
HABs have a direct effect on the coast and its underlying areas. Examples of such
effects include impacts like fishkill (which is caused either by poisoning or oxygen
depletion) and Paralytic Shellfish Poisoning (PSP), a disease in humans caused by the
consumption of tainted shellfish resulting in either partial or complete paralysis of the body
(Villao, 1988). It is these negative effects of HABs that have motivated scientists in multiple
related fields to devote their research efforts on finding methods to reduce HABs.
One method that has not been attempted yet (as far as the group's preliminary
research went) is the use of ultrasound to control HABs. Ultrasound has proven successful as
a method of controlling freshwater algal blooms (caused by cyanobacteria) in agricultural
areas, both locally and overseas (Song, et al., 2005). Removal of cyanobacteria in these
environments is needed due to their oxygen depleting effects with regards to agriculture and
their toxic nature, especially in sources of potable water (Falconer, 1999).
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The use of ultrasound to control freshwater algal blooms employs the concept of microscopic
cavitation resulting from high frequencies, resulting in biological disintegration. Stemming
from this concept, the research will see whether the use of these ultrasound waves can be
applied in the control of HAB's, bringing us to the statement of the problem.
B. Statement of the Problem
This study aims to test whether the exposure of harmful algal blooms (HABs),
specifically those caused by the blooms of the dinoflagellate Pyrodinium bahamense var.
compressum, to ultrasound waves would result in the mitigation or reduction of these
blooms. Assuming this is feasible, the secondary objective of this study is to determine the
ideal length of time it would take for ultrasound exposure to effectively control HABs. The
dinoflagellate’s population size and concentration are aspects that will be observed and
measured during the course of this study. This study also attempts to see whether the
ultrasound transducer to be used in the experiment can easily be deployed on the field,
without necessarily experimenting outside of a controlled laboratory setup. Accomplishing
these goals will lead to the real life problem, which is to find a method of controlling HABs.
C. Significance of the Study
In the research of HAB's, the field of studying Harmful Algal Bloom control has been
progressing far too slowly. Though there are new methods of harmful algal bloom control
(use of chemicals, genetically engineered species, clay flocculation), these methods have
harmful effects on the environment and biological life other than HAB's (Anderson, 2005).
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With the incremental develop of the industry and economy, the HAB (Harmful Algal Bloom)
problems gradually become a cosmopolitan marine disaster, which endangers the health of
the people and the fishery ecosystem (Jinhui, 2005). Fisheries in the Philippines suffer from
fish kills caused by these HAB’s, and the lives of seafaring Filipinos are also more at risk.
Using the methods for HAB control that were mentioned above would only worsen the
problem, highlighting the need for a practical method that will not bring harm to species
other than HABs. This problem is solved by the use of ultrasound to control populations of
HABs, which would also reduce the number of fish kills. This would in turn cause an
increase of the fish supply of our country and decrease the number of fatalities caused by
PSP. Thus, solving this problem would help our country’s poverty problems and its
economic status.
D. Scope and Limitations
The study will be done over a course of around one and a half months. Cultures of
Pyrodinium bahamense var. compressum from the Marine Science Institute (MSI) wasused
in the research study. Twelve groups consisting of two replicates each will be exposed to
different lengths of time. The frequency of ultrasound that was used is 1 MHz. The time of
exposure (independent variable) will vary from each treatment, ranging from 1 hour to 6
hours. The experiment will find out if the optical density, the dependent variable, will
increase, decrease, or remained unchanged. Other than the frequency of the ultrasound, time
of exposure to light, volume of solution, amount of nutrients, salinity, and temperature will
be considered as controlled variables. This study aims to cover the control of the population
of HABs and does not deal with the complete elimination of HABs.
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This study is completely different from the study entitled Using Ultrasound to
Control Algal Blooms which was conducted by Dr. Carl Howard and a team of researchers
from the University of Adelaide. The research of the aforementioned team deals with the
effects of ultrasound to blooms of blue-green algae, whereas this research tests if various
time exposures to ultrasound have an effect on HABs.
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II. REVIEW OF RELATED LITERATURE
A. Harmful Algal Bloom (HAB)
What is a HAB?
An HAB, commonly known as “red tide”, is the discoloration of a body of water
caused by massive populations of coastal dinoflagellates (Villao, 1988). Commonly
distributed in the tropical Indo-Pacific region, HABs are predominant in numerous countries
including the Philippines (Busine, et al., 2003).
Factors affecting HAB growth
Dinoflagellates within HABs prefer high surface-water temperatures and high light
intensities, though this does not mean that HABs only occur in tropical areas. HABs occur in
hot, calm weather because surface temperatures warm up even in normally cool areas
(Badylak, et al., 2004; Maclean, 1977).
Light wind intensity moves the bloom near the coast, whereas strong wind intensity
aids in the swimming of dinoflagellates to the surface. Storms on the other hand, even with
strong wind intensity, disperse the HABs. Storms also result in the death of dinoflagellates
and can prevent the development of red tides (Pollingher & Zenel, 1981).
Red tides usually occur after an upwelling has stopped, but the nutrients brought to
the surface do not appear to be the direct cause of these blooms (Grindley & Nel, 1970). The
overloading of nutrients to bodies of water, or eutrophication, gives favorable conditions to
HABs. The presence of HABs, however, has proved to be detrimental to other organisms in
the environment (Nybakken, 1982).
Effects of HAB to marine and human environment
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HABs have been a significant global and national concern due to their negative public
health and or/economic effects (Fernandez & Ricafrente, 2010). Red tides deplete the
nutrients needed for other marine organisms to survive. They also cause oligotrophication,
which is the abundance of toxic materials in bodies of water. HABs have the ability to
produce very lethal toxins like saxitoxin, Neo-saxitoxin and decarbamoyl, which can cause
the death of marine organisms. These toxins can also accumulate in some animals, and can
result in Paralytic Shellfish Poisoning (PSP) in humans if these animals are eaten. Symptoms
of PSP include paralysis, vomiting, shortness of breath and other difficulties, and can result
in death through respiratory failure (Busine, et al., 2003).
HABs have economic effects on multiple sectors of society. Fish kills caused by
HABs reduce fish supply, while shellfish bans imposed by local authorities caused losses in
the fishing industry, pose problems to international trade, and result in underemployment of
industries (Bajarias, et al., 2003).
Methods of HAB management and monitoring in the Philippines
Current methods of HAB management are limited to detection and analysis of the
areas affected by a bloom, including the implementation of bans on shellfish and similar
products affected, and an information campaign by various government agencies. This
management method has been done since 1984, and is inefficient in the sense that very little
is done to control the bloom physically, and simply involves waiting for it to fade out
(Bajarias, et al., 2006). Other physical means, such as domoic acid treatment, of controlling
and eliminating HABs are still being tested out by various government agencies such as the
PCAMRD (Fernandez & Ricafrente, 2010).
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However, the Philippine government keeps on monitoring seas that are known to
have past cases of red tide. The Department of Health (DOH), and Bureau of Food and Drugs
(BFAD) keeps on acquiring samples of seawater from the seawater to obtain quantitative
analysis of cell density and toxin concentration. Aerial surveillance is also monitored by the
Department of Agriculture (DOA), and Philippine Air Force, to see if there is any
discoloration of the sea’s surface (Busine, et al., 2003).
Methods of HAB management and monitoring outside Philippines
Countries have advanced technologies that the Philippine lacks, and one of them is
the satellite monitoring system (Bajarias et al., 2003). Countries such as China, Norway,
Canada, Japan, and USA use remote sensing satellites to detect HABs. With the use of
satellites, aerial surveillance is much easier (Andersen, et al., 2001; Busine, et al., 2003).
They also train fishermen on how to detect HABs and collect HAB samples with the use of
buoys, lighthouses, and plankton nets. Also, the marine farms are more advanced than in the
Philippines; their fish and mussel farms contain laboratories that separate the poisoned
marine organisms from the healthy ones (Anderson, et al., 2001; Bajarias, et al., 2003).
These countries also developed ways on how to control the population of algae, but
these have limitations: adding of chemicals, flocculation, and biological manipulation.
Adding of chemicals started when the US government added copper sulfate to seas
with HABs near Florida. Adding copper sulfate was effective, but after weeks, the HAB
reestablished itself, killing more fish along the shores of Florida, and calm wind currents also
carried part of the bloom to other seas of United States. They also used other chemicals such
as ozone and aponin, but these have negative effects in marine life other than harmful algae.
Flocculants, substances that capture suspend particles until they become heavy and fall as
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sediments, were tested in Japan and were found to be effective against HABs, but it is very
expensive. Japanese researchers also used the addition of viruses to destroy the algae, and
bacteria, dinoflagellates, and other zooplankton to compete with the algae. It was effective,
but it also massive bivalve and fish kills (Andersen, et al., 2003; Newcombe, 2009).
Pyrodinium bahamense var. compressum
In the Philippines, Pyrodinium bahamense var. compressum has been identified as the
main organism responsible for HAB outbreaks in Manila Bay since 1988. P. bahamense
forms its “blooms” by cell division during their vegetative stage, and is easily grown in a
laboratory setup, given the proper conditions. P. bahamense has a growth rate of one cell
division every three days, and produces a planozygote in later stages of its bloom because of
a union of its gametes. A non-motile hypnozygote is then formed, which brings the organism
into dormancy for about three to four months, unless optimal conditions of salinity,
temperature, and light intensity are established. Once these conditions are met, the
hypnozygotes then germinate via meiosis and then binary fission, in turn initiating a new
bloom (Azanza, 1997).
Blooms of P. bahamense are dominant in Bolinao, Masinloc, Manila, Palawan,
Camiguin, Surigao Province, Leyte, and Samar. These areas are reportedly to have massive
fish kills, especially in the Manila Bay. However, the effects of El Nino and La Nina disrupt
the normal growth pattern of the algae, so fish kills in these areas do not happen at the same
time (Azanza, 1997; Bajarias, et al., 2003; Busine, et al., 2003).
Saxitoxins are considered the most potent neurotoxin found in dinoflagellate blooms
(Busine, et. al., 2003). Aside from Saxitoxin, Pyrodinium also produces other types of
neurotoxins, particularly Neo-saxitoxin, decarbamoyl, gonyautoxin-5 and gonyautoxin-6
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(Busine, et. al., 2003; Corrales, 1991). With these toxins, it is necessary to note that proper
algae culturing protocols would need to be implemented in this research, for the safety of the
researcher (Azanza, 1997).
B. Algal Culture
Factors considered in growing algae
Like all organisms, certain factors should be considered in growing algae. As with all
plants, algae must have sufficient nutrients to support growth, and factors, such as light,
temperature, salinity, seawater quality, mixing and cleanliness will all need to be kept
constant to ensure favorable conditions for algal growth (Food and Agriculture Organization
of the United Nations, 2007; Hallegraeff et al., 1995).
Techniques in growing algae
Aseptic method is strictly imposed when culturing microorganisms. It prevents
addition of unwanted microorganisms. While adding nutrients, or the stock culture, you must
make sure you heat the mouth of the container, or transfer the necessary components near an
open flame (Food and Agriculture Organization of the United Nations, 2007).
In an algal culture system, a stock culture should be maintained. These stock cultures
provide the reservoir of algal cells from which to start the larger-scale cultures used for
feeding. In preparing the replicate culture flasks, use the pipette to transfer a small sample of
the stock culture to the flasks. Use a separate pipette for transferring the nutrients. For
dinoflagellates, their nutrient is F/2 medium, a mixture of vitamins, nitrates, phosphates,
silicates, and other minerals (Food and Agriculture Organization of the United Nations,
2007).
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Algal cultures must be monitored daily to detect if there are dead species, cell
aggregation or clumping, or contaminants. If a culture contains multiple clumped cells, cells
with cell walls broken, more than one species present, or is contaminated with foreign
bodies, the culture should be discarded (Food and Agriculture Organization of the United
Nations, 2007).
Cell counting methods
Monitoring of the algal cultures will also involve a cell count, using either a
haemocytometer or a Sedgewick-Rafter counting slide.
A haemocytometer is widely used by researches because of its easy instructions, its
lightweight use. However, haemocytometer is not suitable for algae larger than 45 microns,
such as P. bahamense. Haemocytometers also rely on calculations and estimation, which can
be inaccurate (Karlson, et al., 2010; Tech Note, 2004).
This research study proposes the Sedgewick-Rafter counting slide, a traditional
counting method. It contains a 20 by 50 grid of 1 mm2 squares. It is recommended with cells
of large size and population. It does not need calculations, but the counting is manual and
time-consuming (Karlson et al., 2010).
Aside from establishing principles and culturing techniques of HABs, this research
will also note the scientific concept of ultrasound and its effects on biological and chemical
materials.
C. Ultrasonic Principles
Basic Ultrasonic Principles
Ultrasound is defined as a high frequency that is above 20 kHz, above the audible
range. Ultrasound waves require an elastic medium, such as solids or liquids, for
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transmission, operated by stressing the medium itself. Its wavelengths are small compared to
audible waves, and it is said to have a “high frequency” relative to the audible range of
humans (Agarwal, 2005).
The most common methods of ultrasonic examination utilize either longitudinal
waves or shear waves, and other forms of sound propagation exist, including surface waves
and Lamb waves. Surface waves are characterized by elliptical particle motions and are
bound to the surface of a material, while Lamb waves are characterized by complex
vibrations in materials where its thickness is less than the ultrasound wave induced to it
(Olympus, 2006).
Ultrasound can be classified into two types: low frequency ultrasound, and high
frequency ultrasound. Low frequency ultrasound ranges from 20 kHz to 1 MHz, and high
frequency ultrasound ranges from 1 MHz onwards (Van Iersel, 2008).
Biological Effects of Ultrasound
There are ways in which ultrasound can produce biological effects such as cavitation,
microstreaming, and heating (Chudleigh & Thilaganathan, 2004). Cavitation is the
ultrasonically induced activity occurring in a liquid or liquid-like material that contains
bubbles or pockets containing gas or vapor (O’Brien, 2007), and can rupture the cell
membranes of microorganisms (Li, 2009). Microstreaming is the formation of small local
fluid circulations, and can be intra- or extracellular. Microstreaming can cause the same
effects to those of cavitation. Heating is caused by the absorption of the ultrasound wave by
organisms, and it can cause internal injuries to the cell (Chudleigh & Thilaganathan, 2004).
Low frequency ultrasound is enough to produce cavitation, microstreaming, and heating in
aquatic environments (O’Brien, 2007; Van Iersel, 2008).
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In tissues of macroscopic animals, high frequency ultrasound can only cause
abrasions in the tissues. Heating and not cavitation is the cause of tissue damage in animals.
As frequency increases, absorption of ultrasound waves increases. As the tissue absorbs the
ultrasound waves, their vibration causes to increase the internal energy of the tissue, which
creates heat (Carstensen, et al., 1974).
Chemical Effects of Ultrasound
In cavitation, the induced activity of bubbles or pockets can grind insoluble
substances in liquid. These insoluble substances will become smaller until it suspends in the
liquid medium (Li, 2009). Ultrasound can also decompose or transform organic molecules,
such as chlorophyll and saxitoxin, into smaller and useless ones. Ultrasound increases the
energy needed to break the bonds between atoms, until the energy reaches the activation
energy, the minimum energy required to have a chemical reaction. Once the organic
molecule changed its form, it can no longer function properly (Emery, et al., 2005; Van
Iersel, 2008). If the harmful algae lacked the necessary compounds needed for
photosynthesis, it can no longer survive (Andersen, et al., 2003).
C. Transducer, the Ultrasound Machine
What is the transducer?
The device that both generates the ultrasound and detects the returning echoes is the
transducer. Transducers are made of materials that exhibit piezoelectricity, which is “electric
polarity due to pressure especially in a crystalline substance” (Fleischer, et al., 1991). In
ultrasonics, the piezoelectric material is the actual transducer because “it converts ultrasound
into electric energy and vice-versa. When voltage is applied, the transducer will expand and
contract, creating ultrasound” (Chudleigh & Thilaganathan, 2004; Sherman & Butler, 2007).
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Main Components of Transducers
There are three main components of transducers, namely the active element, the
backing, and the wear plate. The active element is the piezoelectric material. The backing
acts as an energy conserver by absorbing the energy radiating from the active element.
Finally, the wear plate protects the transducer element from the surroundings (Fleischer, et
al., 1991; Olympus, 2006).
Sonicators
A sonicator is a device used to break open cells using ultrasound waves, a method
called sonication. Sonicators make use of the properties of high frequency ultrasound to
disrupt the cell wall of an organism. Sonication is employed in most studies for extraction of
enzymes within a cell, with insoluble materials separated by centrifugation (Madison Area
Technical College, 2005).
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III. MATERIALS AND METHODS
A. Procurement of Algal Solutions and other materials
A stock culture of Pyrodinium bahamense var. compressum was obtained from the
Marine Science Institute (MSI) at the University of the Philippines (UP) – Diliman Campus.
An ultrasonic cleaner was obtained from the I-MAT Pro Company. The Sedgewick-
Rafter counting slide, materials for the construction of the culture tank and all other
laboratory equipment (stirring rod, pipette, waste bottles, Erlenmeyer flasks, reagent bottles,
F/2 media, microscope, autoclave, Lugol’s Iodine, Eppendorf Tubes, etc.) was obtained from
the MSI. Common materials for cleaning (at the end of the experiment) were bought from
public markets.
B. Preparation and Sterilization of Culture Flasks
Twenty-four (24) 125 mL Erlenmeyer flasks were used in the experiment. A seal for
the flasks were made by rolling a thick sheet of cotton. The roll of cotton was inserted in the
hole of the flask to check if it fits. Otherwise, a portion of cotton must be removed. The
process must be repeated several times until the cotton tightly fits in the hole. Then, the
cotton was wrapped with cheesecloth and twisted to form a handle in the top. The handle was
sealed with masking tape.
Figure 3.2.1. Erlenmeyer flasks obtained in MSI (left picture), and Erlenmeyer flasks were
cotton seal (right picture).
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32 ppt of seawater was filtered by using a water filterer. Seawater must be filtered to
remove unwanted substances (other than salts) (Karlson, et.al, 2010). The filtered seawater
was transferred in a large flask, and each Erlenmeyer flask was filled with 50 mL of filtered
seawater. Then, the seals were covered with aluminum foil.
Figure 3.2.2 Water filterer connected to a container for filtered seawater (left picture).
Erlenmeyer flask filled with filtered seawater (middle picture). Inside the autoclave are
Erlenmeyer flasks with filtered seawater and seals covered with aluminum (right picture).
Autoclaving is necessary to remove unwanted microorganisms inside and outside of
the flask (FAO, 2007). All flasks were placed inside an autoclave for 1 hour and after
autoclaving; they were cooled for the day.
C. Preparation of Algal Solutions
The preparation of algal solutions was executed in a secure, temperature-controlled
room. All stock cultures must be kept in a temperature-controlled room, to control (not alter)
the growth pattern of the algae (Food and Agriculture Organization of the United Nations,
2007; Karlson, et.al, 2010). Aseptic method was used to prevent contamination of unwanted
organisms in the flasks (Food and Agriculture Organization of the United Nations, 2007).
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Figure 3.3.1 Things needed for preparation of algal solutions. From left to right: stock
culture, alcohol lamp, single channel pipette, autoclaved Erlenmeyer flasks with filtered
seawater, and F/2 medium.
F/2 medium must be added to each flask before adding the algae. F/2 medium is a
broth for the algae’s nutrients. Without F/2, the algae will not survive (Food and Agriculture
Organization of the United Nations, 2007). Before adding the F/2, each mouth of the F/2
container and the flask was heated by an alcohol lamp (aseptic methods). A ratio of 1 L of
algal solution to 2 mL of F/2 was used, since this is the protocol MSI imposed on growing P.
bahamense var. compressum. Each flask contained 100 mL of algal solution, so 0.2 mL, or
200 microliters of F/2 was added, by using a single channel pipette. After each flask has been
added with F/2 medium, the mouth of the stock container and the flask was heated, and 50
mL of P. bahamense var. compressum was added, until all 24 flasks were filled. After this,
all flasks were randomized and labeled acc. to their assigned treatment. There were 1 control
and 11 treatments, and each group has two flasks.
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Figure 3.3.2. Aseptic methods for sterilization purposes. Erlenmeyer flask’s mouth was
heated (left), and F/2 container’s mouth was heated (right)
Figure 3.3.3. Transferring of F/2 medium from container to Erlenmeyer flask.
Figure 3.3.4. Transferring stock culture to Erlenmeyer flask near the open flame (aseptic
method).
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The algae will die if there is no light because of absence of photosynthesis
(Hallegraeff et al., 1995). All flasks are kept in the corner of the room near a light source.
Salinity, temperature, light intensity, and wind intensity are the factors to be
considered in the habitat of P. bahamense (Hallegraeff et al., 1995). Salinity was kept
constant by adding the same amount of seawater (in the same concentration of 32 ppt). Since
the flasks are kept in a temperature-controlled room, controlling temperature is not much of
problem. The algae are inside the flasks, which does not have air disturbance. Light intensity
was kept constant by the MSI staff monitoring the time of using the light source in the room.
Figure 3.3.5. All 24 flaks kept near a light source.
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D. Initial Cell Counting
Figure 3.4.1. Things needed for cell counting (from left to right): Eppendorf tubes in orange
case, culture flask, and single channel pipette.
The number of cells in the cleaner tank was counted by using a 20 x 50 Sedgewick-
Rafter counting slide before exposing them in ultrasound waves. A sample of algal solution
was be obtained by using a single channel pipette, and it must be preserved in Lugol’s Iodine
before counting (Karlson, et al., 2010). 1 mL of the solution was obtained at it was
transferred in an Eppendorf tube. Two 1 mL samples were obtained for each flask, because
the counting consists of two trials. Then, each tube was added with 1 drop o f Lugol’s Iodine
by using a dropper. Adding the Lugol’s Iodine was done outside the room since its fumes can
kill the algae (Karlson, et al., 2010).
Then, the 1 mL solution was transferred, by using a different dropper, to the cover
glass of the counting slide. The cover glass must be slowly swung so it completely covers the
solution. Careful alignment of the cover glass will stop air bubbles from proliferating into the
sample and will ensure that the solution is completely spread in the cover glass. If the
solution is completely spread, the slide is ready for counting.
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Figure 3.4.2. Researchers working on cell count while looking in the microscope.
The cover glass of the counting slide was viewed in a microscope using a 10x objective. A
counter was used to aid the researcher in counting cells. While counting, if the researcher
sees “x” cells, he will click the counter “x” times. All 1000 squares wer e checked and the
number of cells was recorded. For faster counting, the squares in the slide were scanned in a
zigzag formation (Karlson et al., 2010).
E. Setting up of ultrasonic cleaner
Figure 3.5. Ultrasonic Cleaner set-up.
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The ultrasonic cleaner served as the culture tank of the experiment, and it was filled
with tap water. Sound waves can pass through solids and liquids, therefore algae can still be
exposed through ultrasound waves (Olympus, 2006). Pyrodinium bahamense var.
compressum can survive in subtle amount of air (Azanza, 1995), so there is no need of
oxygen/carbon dioxide tanks.
2 flasks were placed inside the ultrasonic cleaner. Only the inside of the cleaner must
be wet, and the level of the water must not rise beyond the mark inside the cleaner, to prevent
electrocution (Lee, 2004). If the level of the water goes up beyond the mark, the flasks were
discarded and removed some of the water, until the water level is exactly at the mark.
F. Exposure of Algae to Ultrasound, and Final Cell Counting
After setting up the ultrasonic cleaner, it was switched on. Each treatment was
applied with the same amount of frequency (1 MHz), and with varying amount of time. The
first treatment was exposed with 1 hour of ultrasound. Each succeeding treatment was
exposed with an additional 30 minutes of exposure (90 minutes for the 2nd treatment, 120
minutes for the 3rd, and so on). A countdown timer was used to monitor the time of exposure
for each treatment. At the end of each treatment, the flasks were taken out and the same
process (two trials) was done for counting the algae. After finishing all treatments, the water
inside the cleaner was removed. The cleaner was wiped with tissue until its dry, and it was
kept back in its container.
G. Computation, Graphing, and Tabulation of Collected Data
All data computed or obtained before were presented into tables and graphs using
Microsoft Excel. There will be 12 tables, and each table is assigned for one treatment. The
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table will consist of the initial cell density and final cell density of the treatment. Then, each
table will be interpreted by using line graphs.
H. Statistical Tests (ANOVA and T-Test)
Analysis of Variance (ANOVA) will be used, with a level of significance of 0.05, to
find out if there is a significant difference between the change of cell densities of each
treatment (alternative hypothesis), or if there is no significant difference (null hypothesis). A
t-test will be used, for each treatment with a level of significance of 0.05, to find out if there
is a significant difference between the initial and final cell densities of the treatment
(alternative hypothesis), or if there is no significant difference (null hypothesis).
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IV. BIBLIOGRAPHY
Agarwal, S. K. (2005). Advanced biophysics. New Delhi: APH Publishing. (Agarwal, 2005)
Anderson, M., Andersen, P., Bricelj, V.M., Cullen, J., & Rensel, J. (2003). Monitoring and
management strategies for harmful algal blooms in coastal waters. Paris: UNESCO.
Azanza, M.P., Azanza, R.V., & Ventura, S. (2003). Varied assays for PSP toxins inheatshocked Philippine green mussels (Perna viridis). Journal of food safety, 23, 249-
259.
Azanza, R.V. (1997). Contributions to the understanding of the bloom dynamics of P.
bahamense. Science Diliman, 9(1-2), 1-6.
Azanza, R.V., & Hall, S. (1993). Isolation and culture of Pyrodinium bahamense var.
compressum from the Philippines. USA: Elsevier.
Azanza, R.V., Cruz, L.J., Carino, F.A., Blanca, A.G. & Butardo, V.M. (2009). Paralyticshellfish toxin concentration and cell density changes in Pyrodinium bahamense –
Noctiluca scintillans feeding experiments. Toxicon, 3(109)
Azanza, R.V., Dela Rosa, A., Sombrito, E.Z., Cruz, L., Siringan, F.P., McGlone, M.S.D., &
Duyanen, J. (2001). Harmful algal bloom (HAB) management lessons from
multidisciplinary research program in Manila Bay, Philippines. Philippines: DOST.
Badylak, S., Kelly, K., & Philips, E. (2004). A description of Pyrodinium bahamense
(Dinophyceae) from the Indian River Lagoon, Florida, USA. Phycologia, 43(6), 13-
17.
Bajaras, F., Relox Jr., J., & Fukuyo, Y. (2006). PSP in the Philippines: three decades of monitoring a disaster. Coastal Marine Science, 30(1), 104-106.
Busine, M.B., Cardenas, J., Khonghun, G., Pelobello, M.R., Raymundo, E., & Reyes, C. C.
(2002). The killer tide: The impacts and monitoring of red tide. Ekolohiya, 1(1), 1-8.
Carstensen, E.L., Miller, M.W., & Linke, C.A. (1974). Biological effects of ultrasound.
Journal of Physical Biological Sciences, 2, 173-192.
Cell counting and dye exclusion viability assays using haemocytometer. Tech Note (2004),
3(25), 1-2.
Chudleigh, T., & Thilaganathan, B. (2004). Obstetric ultrasound (3rd Ed.). Philadelphia,
USA: Elsevier Limited.
Emery, R.J., Papadaki, M., Freitas dos Santos, L.M., & Mantzavinos, D. (2005). Extent of
sonochemical degradation and change of toxicity of a pharmaceutical precursor
(triphenylphosphine oxide) in water as a function of treatment conditions.
Environment International, 31, 207-211.
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Falconer, I. R. (1999). An overview of problems caused by toxic blue-green algae
(Cyanobacteria) in drinking and recreational water. Environmental toxicology, 14, 5 –
12.
Fernandez, D., & Ricafrente, M.V. (2010). DOST-PCAMRD supports the PhilHABs
program. The PCAMRD Waves, 1(23), 1-6.
Fleischer, A., Romero, R., Manning, F., Jeanty, P., & James Jr., A.E. (1991). The principles
and practice of ultrasonography in obstetrics and gynecology (4th Ed.). Connecticut,
USA: Prentice-Hall International Inc.
Food and Agriculture Organization of the United Nations. (2007). Installation and operation
of a modular bivalve theory. UK: Author.
Goldman, C.R., & Horne, A.J. (1983). Limnology. California: McGraw-Hill Inc.
Hallegraeff, G.M., Anderson, D.M., Cembella, A.D., & Enevoldsen, H.O. (1995). Manual on
harmful marine microalgae. Place de Fontenoy, Paris: UNESCO.
Karlson, B., Cusack, C., & Bresnan, E. (2010). Microscopic and molecular methods for
quantitative phytoplankton analysis. Place de Fontenoy, Paris: UNESCO.
Jaymalin, M. (1997, May 7). The moribund shellfish industry. The Philippine Star , pp. 1, 17.
Jinhui, W. (2005). The ecological engineering of HAB: Prevention, control, and mitigation of
harmful algal blooms. Electronic Journal of Biology, 1(2), 27-30.
Kinne, O. [Editor], Blaxter, J.H.S., Collier, A.W., Gunkel, W., Helleburst, J.A., & Segal, E.
(1970). Marine ecology, v. 1.Environmental Factors, Part 1. London: Wiley-
Interscience.
Lee, R.L. (1989). Phycology (2nd Ed.). New York: Cambridge University Press.
Lee, S. (2004). Ultrasonic cleaning baths. Retrieved from: http://www.impact
test.com/docs/SV050_055HB.pdf
Li, H., Huai, X., Cai, J, & Liang, S. (2009). Experimental research on antiscale and scale
removal by ultrasonic cavitation. Journal of Thermal Science, 18(1), 65-73.
Maclean, J.L. (1977). Observations on Pyrodinium bahamense plate, a toxic dinoflagellate,
in Papua New Guinea. Limnology and Oceanography. 22(2), 234-254.
Madison Area Technical College, Biotechnology Project. (2005). An overview of sonication.Wisconsin: MATC.
Newcombe, G. (2009). International guide manual for the management of toxic
cyanobacteria. London: GWRC.
Nybakken, J.W. (1982). Marine Biology, an Ecological Approach. New York: Harper &
Row.
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O’Brien, W.D. (2007). Ultrasound-biophysics mechanisms. Progress in Biophysics and
Molecular Biology. Urbana, IL: Elsevier, 93, 212-255.
Olympus (2006).Ultrasonic transducers technical notes. USA: Author.
Oyib, D.H. (2009). Control mechanism of algal growth. Everything About Water ,11, 40-41.
Relox Jr., J., & Bajarias, F. (2003). Harmful algal blooms (HABs) in the Philippines.
Retrieved from: http://fol.fs.a.u-tokyo.ac.jp / /rtw/TOP/EXabst/019JuanRReloxJr.pdf
Ryding, S.O., & Rast, W. (1989). The control of eutrophication of lakes and reservoirs.
Cornforth, UK: Parthenon Publishing Group.
Sassi, J., Viitasalo, S., Rytkonen, J., & Leppakoski, E. (2005). Experiments with ultraviolet
light, ultrasound, and ozone technologies for onboard ballast water treatment.
Finland: Julkaisija-Utgivare.
Sherman, C.H., & Butler, J.L. (2007). Transducers and arrays for underwater sound. New
York: Springer.
Song, W., Teshiba, T., Rein, K., O’shea, K. E. (2005). Ultrasonically induced degradation
and detoxification of Microcystin-LR (cyanobacterial toxin). Environmental science
& technology, 39 (16), 6300 – 6305.
Using ultrasound to control toxic algal blooms. (2010). Retrieved from
http://www.physorg.com/news197715172.html
Usup, G., Kulis, D., & Anderson, D. (1994). Growth and toxin production of the toxic
dinoflagellate Pyrodinium bahamense var. compressum in laboratory cultures.
Natural Toxins, 2, 254-262.
Van Iersel, M.M. (2008). Sensible sonochemistry. Eindhoven: Eindhoven University.
Villao, R.S. (1988). The red tide menace. Diliman Review, 36 (5), 44-45.
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APPENDICES
Appendix A. Summary of Materials and Methods
Figure 5.1. Process Flowchart of the Research Study
Procurement of stock culture
containing P. bahamense var.
compressum (A)
Preparation of culture flasks
containing P. bahamense var.
compressum (n = 24) (B)
Labeling, Grouping, and
Randomization of Solutions (C)
Acquisition of an ultrasonic
sonicator (D
Acquisition of Sedgewick-Rafter slide (E)
Acquisition of other lab equipment (F)
Setting up of Ultrasonic Cleaner (G)
Exposure of Algae to Ultrasound (Algae vs.
Time of Exposure) (I)
Final Cell Counting (2 trials) (J)
Initial Cell Counting (2 trials) (H)
Statistical Tests (ANOVA and T-Test) (L)
Graphing and Tabulation of
Collected Data (K)
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Appendix B. Formulas, Tables, and Graphs needed for Data and Analysis
Table 5.2.1. Table for Analysis of Variance (ANOVA)
Source of
Variation
Sum of
Squares
Degrees of
Freedom
Mean
Square
Fcalc F tab or
Fcrit Treatments SSTr DFTr MSTr
Error SSE DFE MSE
TOTAL SST DFT
∑ ∑
n = Total number of samples nk = Number of samples per treatment
k = Number of Treatments Tk = Treatment Totals
If Fcalc > Ftab , reject null hypothesis. If Fcalc < Ftab, accept null hypothesis.
Table 5.2.2. Table Comparing Initial and Final Cell Density for each Treatment
TREATMENT NO: 1
Flask # Initial Cell Density Final Cell Density Change In Cell Density (D)
21TRIAL 1
TRIAL 2
4TRIAL 1
TRIAL 2
Table 5.2.3. Table for Correlated T-Test
TREATMENT NO: 1
Flask # D D2
21TRIAL 1
TRIAL 2
4TRIAL 1
TRIAL 2
SUMMATION ()
Equations for Correlated T-Test:
∑ ∑ ∑ √ ∑
∑
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n = number of sample pairs = average change in cell density
D = change in cell density ∑ = sum of squares of the difference
= mean difference
If t > tabulated value for t, accept alternative hypothesis, and reject null hypothesis. If t <
tabulated value for t, accept null hypothesis, and reject alternative hypothesis.
Table 5.2.4. Initial, Final, and Change of Cell Densities of Pyrodinium bahamense var.
compressum cultures in Concentration of Algae vs. Time of Exposure
Treatment C T-1 T-2 T-3 T-4 T-5 T-6 T-7 T-8 T-9 T-10 T-11
Flask #
Initial Trial 1
Trial 2
Change Trial 1
Trial 2
Final Trial 1
Trial 2
Legend: All treatments are exposed with 1 MHz ultrasound
C – no exposure to ultrasound T-4 – 2.5 hr of exposure T-8 – 4.5 hr of exposure
T-1 – 1 hr of exposure T-5 – 3 hr of exposure T-9 – 5 hr of exposure
T-2 – 1.5 hr of exposure T-6 - 3.5 hr of exposure T-10 – 5.5 hr of exposure
T-3 – 2 hr of exposure T-7 – 4 hr of exposure T-11- 6 hr of exposure
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Appendix C. Risk Assessment
Table 5.3. Risk Assessment Table
Substance/Device/Organism Risks/Dangerous Effects Safety Procedures
Pyrodinium bahamense var.
compressum
*NOTE: Medical assistance
must be present during
experiment of this kind of
harmful algae.
- Contains saxitoxin (STX), a
dangerous toxin.
- STX can cause gastrointestinal,
respiratory, and neural symptoms.
Symptoms will start by vomiting and
paralysis. Paralysis will be
succeeded by dysphagia, and then
death.
- Fatalities were usually a result of
respiratory failure.
There is no specific antidote for PSP,
and the manner
of treatment is purely symptomatic.
- Before and after handling this
algae, hands must be washed withsoap and water
- Researchers must wear a lab gown,
elbow-length puncture-resistant
gloves, and boots.
- ONLY use mechanical pipetting
for algal transfer
- No eating, drinking, or applying of
cosmetic products during work time.
- Excess algae must be disposed in aleak-proof reagent bottle.
- All other living things unrelated to
the study are prohibited inside the
lab that contains the algae.
Seawater - Slightly hazardous in case of
skin/eye contact (irritant), ingestion,
or inhalation.
- May affect behavior (muscle
spasicity/contraction, somnolence),
sense organs, metabolism, and
cardiovascular system. Continuedexposure may produce dehydration,
internal organ congestion, and coma.
Inhalation: Material is irritating to
mucous membranes and upper
respiratory tract.
- When heated to decomposition it
emits toxic fumes.
- Electrolysis of sodium chloride in
presence of nitrogenous compounds
to produce chlorine may lead to
formation of explosive nitrogen
trichloride. Potentially explosivereaction with dichloromaleic
anhydride + urea.
- Hygroscopic. Reacts with most
nonnoble metals such as iron or
steel, building materials (such as
cement) Sodium chloride is
- Precautions: Keep locked up.. Do
not ingest. Do not breathe dust.
Avoid contact with eyes. Wear
suitable protective clothing. If
ingested, seek medical advice
immediately and show the container
or the label. Keep away from
incompatibles such as oxidizingagents, acids.
- Eye Contact: Check for and
remove any contact lenses. In case
of contact, immediately flush eyes
with plenty of water for at least 15
minutes. Cold water may be used.
Seek medical attention
- Skin Contact: Wash with soap and
water. Cover the irritated skin with
an emollient. Get medical attention
if irritation develops. Cold water
may be used.
- Inhalation: If inhaled, remove to
fresh air. If not breathing, give
artificial respiration. If breathing is
difficult, give oxygen. Get medical
attention if symptoms appear.
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rapidly attacked by bromine
trifluoride. Violent reaction with
lithium.
- Mutagenic for mammalian somatic
cells. Lowest Published Lethal Dose
(LDL) [Man] - Route: Oral; Dose:
1000 mg/kg
-Ingestion: Do NOT induce
vomiting unless directed to do so by
medical personnel. Never give
anything by mouth to an
unconscious person. Loosen tight
clothing such as a collar, tie, belt or
waistband. Get medical attention if
symptoms appear.
- Personal Protection: Splash
goggles. Lab coat. Dust respirator.
Be sure to use an approved/certified
respirator or equivalent. Gloves.
- Accidental Small Spill: Use
appropriate tools to put the spilled
solid in a convenient waste disposal
container. Finish cleaning by
spreading water on the contaminated
surface and dispose of according to
local and regional authorityrequirements.
- Accidental Large Spill: Use a
shovel to put the material into a
convenient waste disposal container.
Finish cleaning by spreading water
on the contaminated surface and
allow evacuating through the
sanitary system.
- Waste Disposal: Waste must be
disposed of in accordance with
federal, state and localenvironmental control regulations.
Lugol’s Iodine - Hazardous in case of ingestion.
Slightly hazardous in case of skin
contact ( irritant, permeator), of eye
contact (irritant).
- Mutagenic for mammalian somatic
cells. Classified Reproductive
system toxin for females. The
substance is toxic to thyroid. The
substance may be toxic to blood,
kidneys, liver, skin, eyes. Repeated
or prolonged exposure to thesubstance can produce target organs
damage.
- Potassium iodide (KI) + Fluorine
Perchlorate (FClO4) will explode on
contact.
- Eye Contact: Check for and
remove any contact lenses. In case
of contact, immediately flush eyes
with plenty of water for at least 15
minutes. Cold water may be used.
Get medical attention.
- Skin Contact: Wash with soap and
water. Cover the irritated skin with
an emollient. Get medical attention
if irritation develops. Cold water
may be used.
- Ingestion: Do NOT induce
vomiting unless directed to do so by
medical personnel. Never give
anything by mouth to an
unconscious person. Loosen tight
clothing such as a collar, tie, belt or
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- Slightly reactive to reactive with
oxidizing agents, reducing agents,
organic materials, metals, acids.
- Acute Potential Health Effects:
Skin: Causes skin irritation. It can
cause brown stains on the skin. It
can be absorbed through the skin.
Eyes: Eye contact with liquid causes
irritation. Iodine vapors may cause
eye irritation. Eye contact with an
excessive amount of iodine vapor
may also cause blepharitis.
Excessive inhalation of iodine
vapors may cause respiratory tract,
nasal, and mucous membrane
irritation. Symptoms may include
coughing, tightness in the chest,
rhinitis, dyspnea/respiratory distress,
coughing, sneezing, pulmonary
edema, chemical pneumonitis,edema of the larynx and bronchi,
pharyngitis, swelling of the parotid
gland, and cachexia. High exposure
may lead to lung disease and may
also affect behavior/central nervous
system (delirium, hallucination,
depression, seizure)
waistband. Get medical attention if
symptoms appear.
- Inhalation: If inhaled, remove to
fresh air. If not breathing, give
artificial respiration. If breathing is
difficult, give oxygen. Get medical
attention.
- Hygienic Practices: Avoid contact
with eyes, skin and clothing. Wash
hands after direct contact. Do not
wear product-contaminated clothing
for prolonged periods.
- Engineering Controls: Provide
exhaust ventilation or other
engineering controls to keep the
airborne concentrations of vapors
below their respective threshold
limit value.
- Personal Protective Equipment:
Splash goggles. Lab coat. Gloves.
- Spill Procedures: Dilute with water
and mop up, or absorb with an inert
dry material and place in an
appropriate waste disposal container.
- Waste Disposal: Dispose of in
accordance with all applicable
federal, state, and local regulations.
Sonicator - Safety concerns relating to
ultrasound technology are possible
noise from the transducer, yet
unknown effects upon humans
affected by the exposure to
ultrasound.
-Heat is generated in the transducer
if the cooling system fails.
- Sonicators are usually constructed
of steel, titanium, aluminium or
ceramic material.
- Sonicators develops noise (if set at
high frequencies) that can irritate
humans and animals (>1 MHz)
- Do not install the sonicator in a
hot/humid area. Place it in an area
with proper ventilation
- Check the connection cable for
damage due to overheating/moisture
- If the generator main fuse blows,
check the generator for a short
circuit, the on/off switch,
connection of the supply
transformer, printed circuits for
blown fuses
- Clean out dirt inside and outside of
the sonicator.
- Wipe/dry ultrasonic cleaner after
use.
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Appendix D. Task List
Table 5.4. Task List of the Methods in the Research Study
ACTIVITYCODE
ACTIVITYDESCRIPTION
OBSERVABLEINDICATORS
PRECEEDINGACTIVITY
ESTIMATEDDURATION
A Procurement of stock culture
containing
Pyrodinium
bahamense var.
compressum
Stock cultureobtained from MSI
B 1
B Preparation of
culture flasks
containing
Pyrodinium
bahamense var.
compressum
Twenty-four 125 mL
Erlenmeyer flasks
with 100 mL AlgalSolutions
C 1
C Labelling,
Grouping, and
Randomization of Solutions
24 flasks are labeled
acc. to where it
belongsFlasks are
randomized using
CRD
G 1
D Acquisition of an
ultrasonic sonicator
Ultrasonic cleaner
obtained from I-MAT Pro Company
c/o Mr. Publico
G 7
E Acquisition of an
Sedgewick-Rafter
silde
Sedgewick-Rafter
slide obtained from
MSI
G 1
F Acquisition of
other lab equipment(beakers, pipette,
droppers,
microscopes,autoclave, etc.)
Microscope, pipette,
autoclave, stirringrod, regeant bottles,
seawater, Eppendorf
tubes, Lugol’sIodine, etc.
G 1
G Setting Up of Ultrasonic Cleaner
Ultrasonic Cleaner isalready switched on
with 2 flasks in a
treatment (Repeated
11 times, one foreach treatment)
H 1
H Initial CellCounting and
Cell Densities of each flask are
I 5
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Computation of
Initial Cell Density
obtained. 2 trials
each
I Exposure of Algae
to Ultrasound
(Algae vs. Time of
Exposure orExperiment A)
All 11 treatments are
done (All flasks
except control are
exposed toultrasound)
J 5
J Final Cell Counting All 1 mL samples of
each flask are
counted (2 trials
each flask)
K 5
K Graphing andTabulation of
Collected Data
Graphs and Tablessaved in Excel
L 1
L Statistical Tests ANOVA, andCorrelated T-Test
performed with 0.05level of significance
_ 1
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Appendix E. Materials Sourcing and Budgeting
Table 5.5.1. Table of Materials needed for Experiment and their Costs
Quantity – MaterialNeeded
Source Address Contact Payment
1 - Autoclave15 - Beaker
1 - Microscope
2 – Single ChannelPipette
24 – 125 mL Erlenmeyer
FlasksBolinao Seawater
Cheesecloth
Cotton
Alcohol Lamp
CHEMICALS:
F/2 medium
Lugol’s Iodine
MarineScience
Institute (MSI)
Velasquez Street, UPDiliman, Quezon City
EsrelitaFlores
921-5967
922-3957
Free of Charge
1 – Ultrasonic Cleaner I-MAT ProCompany
Kentwood Heights,Mariposa Street, Brgy.
Crame, Quezon City
RamonPublico
Free of Charge
1 - Stock culture of
Pyrodinium bahamense
var. compressum
Marine
Science
Institute
Velasquez St., UP
Diliman, Quezon City
Esrelita
Flores
921-5967
922-3957
Free of
Charge
4 – Sedgewick RafterCounting Slides
MarineScience
Institute
Velasquez St., UPDiliman, Quezon City
EsrelitaFlores
921-5967
922-3957
Free of Charge
Table 5.5.2. Table of Transportation and Electricity Consumption
Date of Work Consumption Duration or Price
February 24, 2011
Justin’s Car – Round Trip:
PSHS to MSI
15 minutes
Water Filterer (Useselectricity)
30 minutes
Autoclave (Uses Electricity) 1 hour
February 25, 2011
Commuted: Round Trip:
PSHS to MSI
Taxi – Php 80.00
FX to Agham Road (twice) –
Php 20.00
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Jeep (UP Ikot) – Php 7.00
Jeep (UP to Agham Road) –
Php 10.00
Total: Php 117.00
Microscope Viewing (Uses
Electricity)
2 hours
February 28, 2011 Justin’s Car – Round Trip:PSHS to MSI
15 minutes
Microscope Viewing 2 hours
March 1, 2011 Justin’s Car PSHS to I-MAT Pro
Company – 1 hourI-MAT Pro Company to MSI
(twice) – 30 minutes*2 = 1
hour
MSI to I-MAT Pro Company
– 1 hour
MSI to PSHS = 10 mintuesTotal = 3 hrs. 10 minutes
Microscope Viewing 2 hours
Use of Computer (Letter of
Documentation Editing)
30 minutes
March 4, 2011 Justin’s Car – Round Trip:
PSHS to MSI
15 minutes
Ultrasonic Cleaner 1 hour
Daily Lamp (for Algae Control) 12 hours each day
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Appendix F. Gantt Charts
Figure 5.6. Gantt Chart with Expected Dates of Work
*For legends, see Appendix D (Task List)
Annex E. Network Chart
Figure 5.7. Network Chart of the Research Study
A
B
C
D
E
F
G
H
I
J
K
L
23-Feb 24-Feb 25-Feb 26-Feb 27-Feb 28-Feb 1-Mar 2-Mar 3-Mar 4-Mar 5-Mar 6-Mar 7-Mar 8-Mar 9-Mar 10-Mar 11-Mar 12-Mar 13-Mar 14-Mar 15-Mar
DATE (DAYS)
Feb 23 - START, March 15 - END
1
6
52
3
11
13
7
4
9
12
8
C = 1 d
B = 1 d
A = 1 d E = 1 d
10
D = 7 d
G = 1 d
H = 5 d
I = 5 d
K = 1 d
L = 1 d
F = 1 d
J = 5 d