4. CULTIVATION OF ALGAE (MICROALGAE)

Definition A culture is a genetically homogenous clone propagated from one individual cell or filament in an artificial environment. In theory, culture conditions should resemble the alga’s natural environment as far as possible; in reality many significant differences exist, most of which are deliberately imposed. Basic Culturing Techniques of Microalgae Techniques Basic principles of microbial cultivation in general are applicable to microalgae. The unique ability of microalgae to utilize light energy, however, sets them apart from most microorganisms. The supply of light needs to be satisfied in isolation, cultivation and maintenance of photoautotrophic and mixotrophic microalgae. Isolation of algae Isolation of which involves the following steps: 1. Selection of sources of algae Aquatic algae often appear in planktonic forms. They may be sampled by collecting a representative volume of water. Algae attached to other algae, vascular plants, animals, and rocks, where they can be collected by scraping. 2. Enrichment of a culture Enrichment is the process of providing a suitable environment for the growth and reproduction of a special group of microalgae while being inhibitory or lethal for non-target organisms. 3. Establishing Unialgal Cultures Unialgal cultures contain only one kind of alga but may contain bacteria, fungi, or protozoa. To obtain a unialgal culture one species must be isolated from all the rest; different techniques, some borrowed from microbiology, are available for obtaining unialgal isolates: Streaking and successive plating on agar media Streaking is useful for single-celled, colonial, or filamentous algae that can grow on an agar surface. Following an incubation period, morphologically distinct isolates are picked up and transferred to a fresh agar medium, the processes can be repeated until identical colonies are obtained on a plate. For microalgae obtained from water sources, algal cells can be concentrated by centrifugation, filtration, or sedimentation and then plated on agar medium. An example is to concentrate an aquatic sample on a filter membrane. The membrane is then washed with sterilized water, and the cell suspension transferred to an agar medium with the inoculated side up. After two to three weeks of incubation in this manner, morphologically distinct colonies are picked up under a dissecting microscope and transferred to another agar plate or a sterile liquid medium.

66

FIGURE. An agar plate streaked with a small, green coccoid alga, showing small isolated colonies arising from a single cell. Agar Pour Plates Some algae do not grow on the surface of agar plates, but they do grow embedded in agar. To prepare agar pour plates, cells from the field sample or enrichment culture are mixed with the non-solidified agar and then poured into petri dishes. The non-solidified agar must be cool—only slightly warmer than the gelling point—to avoid overheating and killing the algae. Low-melting-point agar is preferred over normal agar. Direct isolation Filaments can be grabbed with a slightly curved pipette tip and dragged through soft agar (less than 1%) to remove contaminants. It is best to begin with young branches or filament tips. Single-cell isolations using Micropipette Single cells or filaments can be picked up under a dissecting microscope, using micropipettes. The individual cells are transferred to agar medium or fresh sterile medium for isolation.

FIGURE . A pipette is used to remove other small cells (left, middle), leaving the target organism free of contamination (right). This procedure limits the handling of the target organism.

67

FIGURE . Preparation of a micropipette from a Pasteur pipette. (a) The Pasteur pipette is held in the hottest region of the flame, supported on the left by a hand and on the right by forceps. The pipette should be rotated as the glass is heated to a soft, pliable condition. (b) When the glass is soft, the pipette is quickly removed from the flame with a gentle pull to produce a thin tube. (c) The forceps is then relocated to the appropriate region of the thin tube. (d) The forceps is used to gently bend the thin area so that it breaks, forming a micropipette. (e) An enlarged tip of a micropipette, showing a jagged break; this tip is not suitable for use. (f) An enlarged tip with a very smooth break; this tip is suitable for use. Note that the diameter of the tip is larger than the flagellate cell (bearing microscopic scales), thus reducing the probability of shearing as the cell enters the micropipette during isolation.

Atomized Cell Spray Technique A fine or atomized spray of cells can be used to inoculate agar plates. The technique can vary, but in general a liquid cell suspension is atomized with forced sterile air so that cells are scattered onto the plate. For best results, the spray should be administered in a sterile hood or clean environment so that airborne bacteria and fungi are not dispersed onto the plate. The plates are incubated, and after colony formation, selected cells are removed and inoculated as described previously. Serial dilution techniques A simple technique to purify a contaminated strain is to proceed with repeated sub-cultures obtained by progressive dilutions of the original sample. An aliquot is removed from the sample container and placed into a test tube containing sterile medium. After mixing, one aliquot is removed from the test tube and dispensed into multi-wells containing sterile medium, and a second aliquot is removed and added to the middle test tube. After mixing, the process is repeated (i.e., dispensed into multi-wells and added to the test tube on the right). Each cycle dilutes the original sample and increases the probability of single-cell isolation; the cycle stops when it is probable that no cell will be transferred.

68

FIGURE . An illustration of the dilution technique. Zoospores isolation A particularly effective means of obtaining unialgal cultures is isolation of zoospores immediately after they have been released from parental cell walls, but before they stop swimming and attached to a surface. Unlike the surfaces of most algal cells, recently released zoospores are devoid of contaminants, but catching zoospores requires a steady hand and experience. Gravity Separation: Centrifugation, Settling Gravity separation can be effective for partitioning larger and smaller organisms, and the two primary methods are centrifugation and settling. Gravity is perhaps more frequently used to concentrate the target organisms rather than to establish unialgal cultures, but the latter can also be achieved. Usually, the goal is to separate the larger and heavier cells from smaller algae and bacteria. Isolation with Use of Phototaxis Phototaxis has been used to isolate flagellates. This method is effective when the sample contains one dominant flagellate that is a strong swimmer and exhibits phototaxis. In its simplest form, a channel of sterile culture medium or water is created, the sample is added to one end, a focused light source is employed, and the cells swim through the sterile liquid toward or away from the light source (positive or negative phototaxis). Once the cells have moved a sufficient distance into the sterile liquid, they are removed by micropipette and placed into a separate vessel. Isolating Epiphytes After Sonication Epiphytes on larger algae or other organisms are difficult to isolate by direct picking from the host with a micropipette. When the epiphyte is scraped from the host, damage often occurs. Sonication can be employed to vibrate epiphytes from the host, and once suspended, the epiphyte can be picked and handled in the usual way.

69

Isolating Strongly Adhering Organisms Some organisms adhere tightly to surfaces and sonication or more violent mixing may not be appropriate because that one cell may be lost among other materials in the sample before it can be found again and isolated. In this case, the cell can sometimes be washed loose with a stream of water gently blown from a pipette (with a tube and mouthpiece). Once the stream detaches the cell from the substrate and becomes free in the liquid, the cell can be quickly picked, rinsed, and inoculated into the culture medium. Isolating Sand-Dwelling Organisms For sampling, the upper layer of sand is collected with a glass tube, wide-mouthed bottle, or small shovel. The sand and water is placed in a petri dish, and the cells that move up into the overlaying water are either collected with a micropipette or allowed to adhere to floating coverslips. Isolating Cysts from Sediments Sediment samples have substantial amounts of debris that hinder isolation. For flagellates, the sediments can be enriched with nutrients and incubated in the light so that the cysts germinate. Once germinated, cells can be isolated with the techniques described previously. Removing Diatoms with Germanium Dioxide Diatoms can be a problem for other scientists who are attempting to isolate non-diatom algae because they grow very quickly, and can often outcompete other algae. In most cases, the addition of germanium dioxide to the culture leads to the death of most or all diatoms. PRODUCING AXENIC CULTURES While “Unialgal” cultures contain only one kind of alga but may contain bacteria, fungi, or protozoa, axenic cultures should contain only one alga without bacteria, fungi, or protozoa. Biological contamination of algal cultures by other eukaryotes and/or prokaryotic organisms in most cases invalidates experimental work, and may lead to the extinction of the desired algal species in culture through outcompetition or grazing. In practice, it is very difficult to obtain bacteria-free (axenic) cultures, and although measures should be taken to minimize bacterial numbers, a degree of bacterial contamination is often acceptable. While contaminated algal cultures have previously been satisfactory for certain application and experiments, modern experimental methods and application demand that contaminants are not generally present. Hence, for most purposes, algal cultures are maintained as unialgal, contaminant-free or axenic stocks. Although sterile cultures of microalgae may be obtained from specialized culture collections, some of the basic purification techniques are described below.

1. Extensive cell washing Under a dissecting microscope, an individual algal cell is picked up using a micropipette and placed in a sterile liquid medium. The organism is then transferred through a series of sterile media. Associated microorganisms adhering to the algal cells are separated through the action of pipetting and washing off during transfer.

70

2. Density gradient centrifugation Microalgae can be separated from bacteria using density gradient centrifugation. Silica sol, percoll has been used to produce density gradient for the separation of microalgae, where each species is separated into a sharp band. The algae at a particular position within the gradient are collected by fractionation of the gradient. 3. UV irradiation Most algae are slightly more resistant to ultraviolet light than bacterial cells. Thus, following UV irradiation, washing and diluting a sample, then spraying or streaking it on selective agar medium may produce pure algal culture free of bacteria. 4. Filtration Algae can be separated from bacteria using membrane filters. Sonication is often employed to break up the algae into small length filaments (3–5 cells). The diluted sample is then vacuum filtered. 5. Antibiotics Antibiotics discourage growth of contaminating cyanobacteria and other bacteria in algal culture, For example: • Imipenem (110 µgml_1) was used to purify unicellular eukaryotic microalgae. • The antibiotics nystatin (100 µgml_1) and cycloheximide (100 µgml_1) were used

to eliminate fungal contaminants. • Best results appear to occur when an actively growing culture of algae is exposed

to a mixture of penicillin, streptomycin, and gentamycin for around 24 h. This drastically reduces the growth of bacteria while allowing the microalgae to continue to grow, increasing the chances of obtaining an axenic cell when using micropipette or agar streaking isolation

• Other antibiotics that can be used include chloramphenicol, tetracycline, and bacitracin..

Different algal species tolerate different concentrations of antibiotics, so a range of antibiotic concentrations should be used (generally 50–500‰ w/v) and then select the culture that has surviving algal cells but no surviving bacteria or other contaminants Antibiotic solutions should be made with distilled water and filter-sterilized (0.2 µm filter units) into sterile tubes, and should be stored frozen until use. 6. Bleach Resistant stages such as zygotes or akinetes can be treated with bleach to kill epiphytes, then planted on agar for germination. It is usually necessary to try several different concentrations of bleach and times of exposure to find a treatment that will kill epiphytes without harming the alga. Checking the Sterility of cultures Sterility of cultures should be checked by microscopic examination (phase contrast) or by adding a small amount of sterile bacterial culture medium (e.g., 0.1% peptone) to a microalgal culture, incubated in dark and observing regularly for two to three days for bacterial growth. There should be no indications of any microbial growth. Absence of bacterial growth does not, however, ensure that the microalgal culture is axenic, because the majority of bacteria do not respond to standard enrichments. In reality there is no way of demonstrating that a microalgal culture is completely axenic.

71

Maintenance and preservation of microalgal strains Algal strains can be maintained in liquid or on solid agar media. Some species of algae can be kept in liquid nitrogen for long-term storage. Stock cultures Handling Algal strains should be carefully protected against contamination during handling To reduce risks, two series of stocks are often retained, one which supplies the starter cultures for the production system and the other which is only subjected to the handling necessary for maintenance. Stock cultures are kept in test-tubes at low light intensity and a temperature. Constant illumination is suitable for the maintenance of flagellates, but may result in decreased cell size in diatom stock cultures. Stock cultures are maintained for about a month and then transferred to create a new culture line. CULTURE PARAMETERS A culture has three distinct components: (1) a culture medium contained in a suitable vessel; (2) the algal cells growing in the medium; (3) air, to allow exchange of carbon dioxide between medium and atmosphere. For an entirely autotrophic alga, all that is needed for growth is light, CO2, water, nutrients, and trace elements. By means of photosynthesis the alga will be able to synthesize all the biochemical compounds necessary for growth. Only a minority of algae is, however, entirely autotrophic; many are unable to synthesize certain biochemical compounds (certain vitamins, e.g.) and will require these to be present in the medium (obligate mixotropy condition). The most important parameters regulating algal growth are nutrient quantity and quality, light, pH, turbulence, salinity, and temperature. The most optimal parameters as well as the tolerated ranges are species specific and the various factors may be interdependent and a parameter that is optimal for one set of conditions is not necessarily optimal for another. Temperature The temperature at which cultures are maintained should ideally be as close as possible to the temperature at which the organisms were collected; polar organisms (20οC). Most commonly cultured species of microalgae tolerate temperatures between 16 and 27οC, although this may vary with the species, and strain cultured. An intermediate value of 18–20οC is most often employed. Temperatures lower than 16οC will slow down growth, whereas those higher than 35οC are lethal for a number of species. Light Light is the source of energy which drives photosynthetic reactions in algae and in this regard intensity, spectral quality, and photoperiod need to be considered. Light intensity plays an important role, but the requirements greatly vary with the culture depth and the density of the algal culture: at higher depths and cell concentrations the light intensity must be increased to penetrate through the culture. Too high light intensity (e.g., direct sunlight, small container close to artificial light) may result in photoinhibition. Moreover, overheating due to both natural and artificial illumination should be avoided. Light may be natural or supplied by fluorescent tubes. Fluorescent tubes emitting either in the blue or the red light

72

spectrum can be used, as these are the most active portions of the light spectrum for photosynthesis. Light intensity and quality can be manipulated with filters. Many microalgal species do not grow well under constant illumination, and hence a light/dark (LD) cycle is used (maximum 16:8 LD, usually 14:10 or 12:12). PH The pH range for most cultured algal species is between 7 and 9, with the optimum range being 8.2–8.7, though there are species that dwell in more acid/basic environments. Complete culture collapse due to the disruption of many cellular processes can result from a failure to maintain an acceptable pH. The latter is accomplished by aerating the culture. In the case of high-density algal culture, the addition of carbon dioxide allows to correct for increased pH, which may reach limiting values of up to pH 9 during algal growth. Salinity Marine algae are extremely tolerant to changes in salinity. Most species grow best at a salinity that is slightly lower than that of their native habitat, which is obtained by diluting sea water with tap water. Salinities of 20–24 g l-1 are found to be optimal. Mixing Mixing is necessary • to prevent sedimentation of the algae, • to ensure that all cells of the population are equally exposed to the light and

nutrients, to avoid thermal stratification (e.g., in outdoor cultures), • to improve gas exchange between the culture medium and the air. For very dense

cultures, the CO2 originating from the air (containing 0.03% CO2) bubbled through the culture is limiting the algal growth and pure carbon dioxide may be supplemented to the air supply (e.g., at a rate of 1-5% of the volume of air). CO2 addition furthermore buffers the water against pH changes as a result of the CO2/HCO-3 balance.

It should be noted that in the ocean cells seldom experience turbulence, and hence mixing should be gentle. Culture vessels Culture vessels should have the following properties: • non-toxic (chemically inert); • reasonably transparent to light; • easily cleaned and sterilized; and • provide a large surface to volume ratio (depending on the organism). MEDIA CHOICE AND PREPARATION When choosing a culture medium, the natural habitat of the species in question should be considered in order to determine its environmental requirements. Media can be classified as being defined or undefined.

Defined media, which are often essential for nutritional studies, have constituents that are all known. Undefined media, on the other hand, contain one or more natural or complex ingredients, for example, agar or liver extract and seawater, the composition of which is unknown and may vary.

73

Media may be prepared by combining concentrated stock solutions, which are not combined before use, to avoid precipitation and contamination. Reagent grade chemicals and bidistilled (or purer) water should be used to make stock solutions of enrichments. Gentle heating and/or magnetic stirring of stock solutions can be used to ensure complete dissolution. When preparing a stock solution containing a mixture of compounds, each compound has to be dissolved individually in a minimal volume of water before mixing, then combined with the other and the volume diluted to the needed amount. Stock solution should be stored at low temperature in tightly sealed glassware, because evaporation may alter initial concentrations. MARINE MEDIA Seawater is an ideal medium for growth of marine species, but it is an intrinsically complex medium, containing over 50 known elements in addition to a large but variable number of organic compounds. Media for the culture of marine phytoplankton consist of a seawater base which may be supplemented by various substances essential for microalgal growth, including nutrients, trace metals and chelators, vitamins, soil extract, and buffer compounds. The salinity of the seawater base should first be checked (30–35‰ for marine phytoplankton), and any necessary adjustments (addition of fresh water/evaporation) made before addition of enrichments. Seawater, stock solutions of enrichments, and the final media must be sterile in order to prevent (or more realistically minimize) biological contamination of unialgal cultures. Autoclaving is a process which has many effects on seawater and its constituents:

• Potentially altering or destroying inhibitory organic compounds, as well as beneficial organic molecules.

• Because of the steam atmosphere in an autoclave, CO2 is driven out of the seawater and the pH is raised to about 10, a level which can cause precipitation of the iron and phosphate added in the medium. Some of this precipitate may disappear upon

(1) re-equilibriation of CO2 on cooling, but the reduced iron and phosphate levels may limit algal growth. (2) The presence of ethylenediaminetetraacetic acid (EDTA) and the use of organic phosphate may reduce precipitation effects. (3) Addition of 5% or more of distilled water may also help to reduce precipitation (but may affect final salinity). (4) The best solution, however, if media are autoclaved, is to sterilize iron and phosphate (or even all media additions) separately and add them aseptically afterwards.

Agar medium Some marine microalgae grow well on solid substrate. A 3% high grade agar can be used for the solid substrate. The agar and culture medium however should not be autoclaved together, because toxic breakdown products can be generated. The best procedure is to autoclave 30% agar in deionized water in one container and nine times as much seawater base in another. After removing from the autoclave, sterile nutrients are added aseptically to the water, which is then mixed with the molten agar. After mixing, the warm fluid is poured into sterile Petri dishes, where it solidifies when it cools.

74

Seawater Base The quality of water used in media preparation is very important. 1. Natural seawater can be collected near shore, but its salinity and quality is often quite variable and unpredictable, due to anthropogenic pollution, toxic metabolites released by algal blooms in coastal waters. The quality of coastal water may be improved by

− ageing for a few months at 4οC (allowing bacteria degradation), − by autoclaving (heat may denature inhibitory substances), − or by filtering through acid-washed charcoal (which absorbs toxic organic

compounds). − Filtering through filter papers. Most coastal waters contain significant

quantities of inorganic and organic particulate matter, and therefore must be filtered before use (e.g., Whatman no. 1 filter paper).

The low biomass and continual depletion of many trace elements from the surface waters of the open ocean by biogeochemical processes makes this water much cleaner, and therefore preferable for culturing purposes. Seawater should be stored in cool dark conditions. 2. Artificial seawater, made by mixing various salts with deionized water. Artificial or synthetic seawter has the advantage of being entirely defined from the chemical point of view, but it is very laborious to prepare, and often does not support satisfactory algal growth. Trace contaminants in the salts used are at rather high concentrations in artificial seawater because so much salt must be added to achieve the salinity of full strength seawater.

3. Commercial preparations are available, which consists of synthetic mixes of the major salts present in natural sea water, such as Tropic Marine Sea Salts produced in Germany for Quality Marine (USA) and Instant Ocean Sea Salts by Aquarium System (USA). Nutrients The term ‘nutrient’ is colloquially applied to a chemical required in relatively large quantities, but can be used for any element or compound necessary for algal growth.

75

The average concentrations of constituents of potential biological importance found in typical seawater are summarized in Table 6.10.

These nutrients can be divided into three groups, I, II, and III; with decreasing concentration: • Group I. Concentrations of these constituents exhibit essentially no variation in

seawater, and high algal biomass cannot deplete them in culture media. These constituents do not, therefore, have to be added to culture media using natural seawater, but do need to be added to deionized water when making artificial seawater media.

76

• Group II. Also have quite constant concentrations in seawater. Because microalgal biomass cannot deplete their concentrations significantly, they also do not need to be added to natural seawater media. Standard artificial media (and some natural seawater media) add molybdenum (as molybdate), an essential nutrient for algae, selenium (as selenite), which has been demonstrated to be needed by some algae. Strontium, bromide, and flouride, all of which occur at relatively high concentrations in seawater and none of which have been shown to be essential for microalgal growth.

• Group III. All known to be needed by microalgae (silicon is needed only by diatoms and some chrysophytes, and nickel is only known to be needed to form urease when algae are using urea as a nitrogen source). These nutrients are generally present at low concentrations in natural seawater, and because microalgae take up substantial amounts, concentrations vary widely. All of these nutrients (except silicon and nickel in some circumstances) generally need to be added to culture media in order to generate significant microalgal biomass.

Nitrate is the nitrogen source most often used in culture media, but ammonium can also be used, and indeed is the preferential form for many algae because it does not have to be reduced prior to amino acid synthesis. Ammonium concentrations greater than 25 µM are, however, often reported to be toxic to phytoplankton, so concentrations should be kept low. Inorganic (ortho) phosphate, the phosphorus form preferentially used by microalgae, is most often added to culture media, but organic (glycero) phosphate is sometimes used, particularly when precipitation of phosphate is anticipated (when nutrients are autoclaved in the culture media rather than separately). Most microalgae are capable of producing cell surface phosphatases, which allow them to utilize this and other forms of organic phosphate as a source of phosphorus. The trace metals that are essential for microalgal growth are incorporated into essential organic molecules, particularly a variety of coenzyme factors that enter into photosynthetic reactions. Of these metals, the concentrations of Fe, Mn, Zn, Cu and Co (and sometimes Mo and Se) in natural waters may be limiting to algal growth. Chelators are chemical molecules that complex with metals and influence the biological availability of these metals. Chelators act as trace metal buffers, maintaining constant concentrations of free ionic metal. It is the free ionic metal, not the chelated metal, which influences microalgae, either as a nutrient or as a toxin. Without proper chelation some metals (such as Cu) are often present at toxic concentrations, and others (such as Fe) tend to precipitate and become unavailable to phytoplankton. In natural seawater, dissolved organic molecules (generally present at concentrations of 1–10 mg l-1) act as chelators. The most widely used chelator in culture media additions is EDTA, which must be present at high concentrations because most complexes with Ca and Mg, present in large amounts in seawater. EDTA may have an additional benefit of reducing precipitation during autoclaving. High concentrations have, however, occasionally been reported to be toxic to microalgae. As an alternative the organic chelator citrate is sometimes utilized. The ratio of chelator:metal in culture medium ranges from 1:1 in f/2 to 10:1 in K medium. High ratios may result in metal deficiencies for microalgae (i.e., too much metal is complexed), and thus many media therefore use intermediate ratios.

77

Vitamins Roughly all microalgal species tested have been shown to have a requirement for vitamin B12 (cobalamin), which appears to be important in transferring methyl groups and methylating toxic elements such as arsenic, mercury, tin, thallium, platinum, gold, and tellurium, around 20% need thiamine (vitamin B1), and less than 5% need biotin (vitamin H). It is recommended that these vitamins are routinely added to culture media. Soil Extract Soil extract has historically been an important component of culture media. It is prepared by heating, boiling, or autoclaving a 5–30% slurry of soil in fresh water or seawater and subsequently filtering out the soil. The solution provides macronutrients, micronutrients, vitamins, and trace metal chelators in undefined quantities, each batch being different, and hence having unpredictable effects on microalgae. With increasing understanding of the importance of various constituents of culture media, soil extract is less frequently used. Buffers The control of pH in culture media is important because

− certain algae grow only within narrowly defined pH ranges − in order to prevent the formation of precipitates.

Except under unusual conditions, the pH of natural seawater is around 8. Because of the large buffering capacity of natural seawater due to its bicarbonate buffering system it is quite easy to maintain the pH of marine culture media. The buffer system is overwhelmed only

− during autoclaving, when high temperatures drive CO2 out of solution and hence cause a shift in the bicarbonate buffer system and an increase in pH, or

− in very dense cultures of microalgae, when enough CO2 is taken up to produce a similar effect.

As culture medium cools after autoclaving, CO2 reenters solution from the atmosphere, but certain measures must be taken if normal pH is not fully restored:

• The pH of seawater may be lowered prior to autoclaving (adjustment to pH 7–7.5 with 1 M HCl) to compensate for subsequent increases.

• Certain media recipes include additions of extra buffer, either as bicarbonate, Tris (Trishydroxymethyl-aminomethane), or glycylglycine to supplement the natural buffering system. Tris has occasionally been cited for its toxic properties to microalgae such as Haematococcus sp. Glycylglycine is rapidly metabolized by bacteria and hence can only be used with axenic cultures. These additions are generally not necessary if media are filter sterilized, unless very high cell densities are expected.

• The problem of CO2 depletion in dense cultures may be reduced by having a large surface area of media relative to the volume of the culture, or by bubbling with either air (CO2 concentration ca. 0.03%) or air with increased CO2 concentrations (0.5–5%). Unless there is a large amount of biomass taking up the CO2, the higher concentrations could actually cause a significant decline in pH. When bubbling is employed, the gas must first pass through an inline 0.2 µm filter unit (e.g., Millipore Millex GS) to maintain sterile conditions. For many microalgal species, aeration is not an option because the physical disturbance may inhibit growth or kill cells.

78

Some of the most commonly used freshwater media, defined and undefined, are listed in Table 6.2–Table 6.9.

79

80

81

82

Some of the most commonly used marine media, defined and undefined, are listed in Table 6.11–Table 6.17.

83

84

85

86

Table 6.18 summarizes the algal classes that have been successfully cultured and their corresponding media names. For a full range of possible media refer to the catalog of strains from culture collections present all over the world such as:

• UTEX (Culture Collection of Algae at the University of Texas at Austin, http://www.bio.utexas.edu/research/utex/)

• CCAP (Culture Collection of Algae and Protozoa, Argyll, Scotland, http://www.ife.ac.uk/ccap/)

• UTCC (University of Toronto Culture Collection of Algae and Cyanobacteria, http://www.botany.utoronto.ca/utcc/)

• CCMP (The Provasoli-Guillard National Center for Culture of Marine Phytoplankton, Maine, http://ccmp.bigelow.org/)

• CSIRO (CSIRO Collection of living microalgae, Tasmania, http://www.marine.csiro.au/ microalgae/collection.html).

STERILIZATION OF CULTURE MATERIALS Sterilization can be defined as a process which ensures total inactivation of microbial life, and should not be confused with disinfection, which is defined as the reduction of bacterial numbers. The primary purpose of sterilization is to prevent contamination by unwanted organisms, but it may also serve to eliminate unwanted chemicals. Several methods are available for sterilization of material, some of which can be used also for growth media: • Autoclaving (moist heat) is the most widely used technique for sterilizing culture

media and vessels, and is the ultimate guarantee of sterility (including the destruction of viruses). A commercial autoclave is the best, but pressure cookers of various sizes are also suitable.

87

http://ccmp.bigelow.org/http://www.marine.csiro.au/

Sterility requires 15 min at 1–2 Bar pressure and a temperature of 121οC in the entire volume of the liquid (i.e., longer times for larger volumes of liquid; approximately 10 min for 100 ml, 20 min for 2 l, 35 min for 5 l). Flasks containing media should not be more than half full, and should be left partially open or plugged with cotton wool or covered with aluminium foil or paper, because for sterility the steam must penetrate the material. Autoclave steam may introduce chemical contaminants; empty glass and polycarbonate vessels should be autoclaved containing a small amount of bidistilled water which is poured out (thus diluting contaminants) under sterile conditions prior to use. Vessels should never be closed, because of the risk of implosion, by using cotton wool bungs, or by leaving screw caps slightly open. Ensure that heating elements of the autoclave are covered with distilled water, and the escape valve should not be closed until a steady stream of steam is observed. After autoclaving, the pressure release valve should not be opened until the temperature has cooled to below 80οC. Autoclave steam may contaminate the media (i.e., with trace metals from the autoclave tubing). Autoclaving also produces leaching of chemicals from the medium receptacle into the medium (silica from glass bottles, toxic chemicals from plastics). Autoclaving in well-used Teflon or polycarbonate vessels reduces leaching of trace contaminants.

• Sterile filtration is probably the best method of sterilizing media without altering their chemistry. Membrane filters of 0.2 µm porosity are generally considered to yield water free of bacteria, but not viruses. 0.1 µm filters can be used, but the time required for filtration of large volumes of culture media may be excessively long. Vitamin stock solutions are routinely filtered through 0.2 µm single use filter units (e.g., Millipore Millex GS), because heat sterilization will denature these organic compounds.

In order to minimize effects of any microbial contaminations, all stock solutions should be stored in a refrigerator at 4οC, except vitamin stocks which are stored frozen at –20οC and thawed immediately prior to use. CULTURE METHODS

Algae can be produced according to a great variety of methods. The terminology used to describe the type of algal culture include: − Indoor/Outdoor. Indoor culture allows control over illumination, temperature,

nutrient level, contamination with predators and competing algae, whereas outdoor algal systems though cheaper, make it very difficult to grow specific algal cultures for extended periods.

− Open/Closed. Open cultures such as uncovered ponds and tanks (indoors or outdoors) are more readily contaminated than closed culture vessels such as tubes, flasks, carboys, bags, etc.

− Axenic (=sterile)/Xenic. Axenic cultures are free of any foreign organisms such as bacteria, but this cultivation is expensive and difficult, because it requires a strict sterilization of all glassware, culture media and vessels to avoid contamination. These constraints make it impractical (and very expensive) for commercial operations. On the other hand, non-axenic or xenic cultivation, though cheaper and less laborious, are more prone to crash, less predictable, and often of inconsistent quality.

− Batch, Continuous, and Semi-Continuous. These are the three basic types of algal culture which will be described in the following sections.

88

BATCH CULTURES This is the most common method for cultivation of microalgal cells. The batch culture consists of a single inoculation of cells into a container of fertilized seawater followed by a growing period under favorable conditions for several days and finally harvesting when the algal population reaches its maximum or near-maximum density. Some form of agitation, such as shaking or impeller mixing, is necessary to ensure nutrient and gaseous exchange at the cell–water interface. The culture vessel can be a simple conical flask or an environment controlled reactor. In a photosynthetic or mixotrophic culture, CO2 is supplied by either purging the conical flask with CO2 enriched air (e.g. 5%v/v CO2 in air) and capped, or by gassing the culture continuously with CO2 enriched air. The culture can be illuminated externally by either natural or artificial light sources, or sunlight through optical fiber, placed in the culture vessels. Batch culture, is a volume-limited system, in which there is no input or output of materials, that is, resources are finite. The algal population cell density increases constantly, whereas other nutrient components of the culture medium decrease over time until the exhaustion of some limiting factor. Any products produced by the cells during growth also increase in concentration in the culture medium. Once the resources have been utilized by the cells, the cultures die unless supplied with new medium. In practice this is done by subculturing, that is, transferring a volume of existing culture to a large volume of fresh culture medium at regular intervals prior to reaching the stationary phase and the larger culture volumes are then brought to a maximum density and harvested. Batch culture systems are widely applied because of their advantages which include: • Ease of operation and simplicity • Flexibility, allowing to change species • allowing to remedy defects in the system rapidly. Although often considered as the most reliable method, batch culture is not necessarily the most efficient method. Disadvantages • Batch cultures are harvested just prior to the initiation of the stationary phase and

must thus always be maintained for a substantial period of time. • The quality of the harvested cells may be less predictable than that in continuous

systems and for example vary with the timing of the harvest. • Another disadvantage is the need to prevent contamination during the initial

inoculation and early growth period. Because the density of the desired microalgae is low and the concentration of nutrients is high, any contaminant with a faster growth rate is capable of outgrowing the culture.

• Batch cultures also require a lot of labor to harvest, clean, sterilize, refill, and inoculate the containers.

POPULATION DYNAMICS

Batch culture systems can be described by different phases, reflecting changes in the biomass and in its environment. Algal population shows a typical pattern of growth according to a sigmoid curve (Figure 6.1), consisting of a succession of six phases, characterized by variations in the growth rate; the six phases are summarized in Table 6.19.

89

1. Lag phase An initial lag or induction phase, where, just after the inoculum. In this phase the cells begin to absorb the nutriens supplied with the culture medium and increase in size, but not in number, and the specific growth rate is at the sub-maximum level. The growth lag could be due to the presence of non-viable cells or spores in the inoculum or may be viable, but not in condition to divide. The lag in growth could be also attributed to the physiological adaptation of the cell metabolism to growth, such as the increase of the levels of enzymes and metabolites involved in cell division and carbon fixation. Cultures inoculated with exponentially growing algae have short lag phases, which can seriously reduce the time required for upscaling. 2. Acceleration growth phase At the late lag phase, the cells have adjusted to the new environment and begin to grow and multiply in accelerating growth phase. 3. Exponential phase After the accelerating phase, the cells enter the exponential (or logarithmic) growth phase. At this phase, cells grow and divide as a function of time according to the exponential function:

where N2 and N1 are the number of cells at two successive times and µ is the growth rate. During this phase, the growth rate reached is kept constant.

Time

FIGURE 6.1 Growth curve of an algal population under batch culture conditions.

90

4. Retardation phase In retardation phase, cell growth rate decreases because mainly light (shading effect of algae), but also nutrients, pH, carbon dioxide, and other physical and chemical factors begin to limit growth. Following this phase, the cell population continues to increase, but the growth rate decreases until it reaches zero, at which point the culture enters the stationary phase. 5. The stationary phase During which the cell concentration remains constant at its maximum value. 6. Crash phase The final stage of the culture is the death or “crash” phase, characterized by a negative growth rate; during this phase water quality deteriorates, mainly due to catabolite accumulation, and nutrients are depleted to a level incapable to sustain growth. Cell density decreases rapidly and the culture eventually collapses. In practice, culture crashes can be caused by a variety of reasons, including the depletion of a nutrient, oxygen deficiency, overheating, pH disturbance, or contamination. The key to the success of algal production is maintaining all cultures in the exponential phase of growth. Also, the nutritional value of the produced algae is inferior once the culture is beyond Phase 4 due to

1. reduced digestibility, 2. deficient composition, 3. and possible production of toxic metabolites.

Upscaling culture conditions The upscaling of microalgae production starts from small containers (0.5 ml) and proceeds through various steps up to the mass production in Polyethylene bags (up to 450 liter). Each step involves an increase of the culture volume: when mature, the algal population of a smaller volume is sacrificed to replicate the same vessel and to inoculate larger vessels. According to the algal concentration, the volume of the inoculums amounts to 2-10% of the final culture volume. The following consecutive stages might be utilized: test tubes, 2 l flasks, 5 and 20 l carboys, 160 l cylinders, 500 l indoor tanks, 5,000 l to 25,000 l outdoor tanks.

Fig A typical scheme of a batch type production

91

CONTINUOUS CULTURES In continuous cultures, cultures are maintained at a chosen point on the growth curve by the regulated addition of fresh culture medium. In practice, a volume of fresh culture medium is added automatically at a rate proportional to the growth rate of the alga, while an equal volume of culture is removed. This method of culturing algae permits the maintenance of cultures very close to the maximum growth rate, because the culture never runs out of nutrients.

Fig. . Schematic diagram of a chemostat setup.

In continuous culture system, nutrients are supplied to the cell culture at a constant rate, and in order to maintain a constant volume, an equal volume of cell culture is removed. This allows the cell population to reach a “steady state” (i.e., growth and cell division where the growth rate and the total number of cells per milliliter of culture remains constant).

Two categories of continuous cultures can be distinguished:

• Turbidostat culture, in which fresh medium is delivered only when the cell density of the culture reaches some predetermined point, as measured by the extinction of light passing through the culture. At this point, fresh medium is added to the culture and an equal volume of culture is removed. The diluted culture increases in cell density until the process is repeated.

• Chemostat culture (constant chemical environment), in which a flow of fresh medium is introduced into the culture at a steady, predetermined rate, in this way the growth rate is kept constant. In many chemostat continuous culture systems, the rate of media flow can be adjusted, and is often set at approximately 20% of culture volume per day.

92

Advantages of continuous cultures • Continuous cultures have the advantages of producing algae of more predictable

quality. • They are amenable to technological control and automation, which in turn

increases the reliability of the system and reduces the need for labor Disadvantages of continuous cultures The disadvantages of the continuous system are

• Its relatively high cost and complexity. • The requirements for constant illumination and temperature mostly restrict

continuous systems to indoors and this is only feasible for relatively small production scales.

SEMI-CONTINUOUS CULTURES In a semi-continuous system the fresh medium is delivered to the culture all at once, by simply opening a valve in the medium delivery line. Fresh medium flows into the culture vessel, and spent culture flows out into a collecting vessel. Once the required medium has entered the culture, the valve is closed, and the culture is allowed to grow for 24 h, when the procedure is repeated. Competitors, predators, or contaminants and metabolites eventually build up, rendering the culture unsuitable for further use. As the culture is not harvested completely, the semicontinuous method yields more algae than the batch method for a given tank. COMMERCIAL-SCALE CULTURES Cultivation of microalgae for commercial purposes is presently carried out, with only a few exceptions, in open systems. A number of types of ponds have been designed and experimented with for microalgae cultivation. They vary in size, shape, material used for construction, type of agitation and inclination.

1. Circular ponds 2. Raceway ponds 3. Inclined systems (sloping cascade)

Fig. Illustration of algal mass culture systems

93

The nutrient medium for outdoor cultures The nutrient medium for outdoor cultures is based on that used indoors, but agricultural-grade fertilizers are used (nitrate and phosphate fertilizers and a few other micronutrients) instead of laboratory-grade reagents. Cultures from indoor production may serve as inoculum for monospecific cultures.

Outdoor advantages/disadvantages Advantages Algal production in outdoor ponds are easier and inexpensive to build and operate. Disadvantages

• Algae cannot be maintained for prolonged period • Outdoor culture is only suitable for a few, fast-growing species due to

problems with contamination by predators, parasites, and more opportunistic algae that tend to dominate regardless of the species used as inoculum.

• Outdoor production is often characterized by a poor batch to batch consistency • Unpredictable culture crashes could be caused by changes in weather,

sunlight, or water quality. At present, large-scale commercial production of microalgae biomass is limited to Dunaliella, Haematococcus, Arthrospira, and Chlorella, which are cultivated in open ponds at farms located around the world. These algae are a source for viable and inexpensive carotenoids, pigments, proteins, and vitamins that can be used for the production of nutraceuticals, pharmaceuticals, animal feed additives, and cosmetics. Lakes and natural ponds When microalgae find suitable climatic conditions and sufficient nutrients, they grow profusely. If the chemical characteristics of the water are selective, for example, due to high pH or high salinity, the bloom is almost monospecific. There are many examples of eutrophic lakes or small natural basins exploited for microalgae production.

94

Fig . (a) A Kanembu woman harvesting Arthrospira platensis from lake Kossorom, a permanent alkaline lake at the north-east fringe of lake Chad (Chad).; (b) Harvesting of Arthrospira from an old volcanic crater filled with alkaline water in Myanmar. PHOTOBIOREACTORS (PBR) Definition of photobioreactors Photobioreactors can be defined as closed culture systems for phototrophs in which a great proportion of the light (>90%) has to pass through the transparent reactor’s walls to reach the cultivated cells. Advantages − PBR do not allow, or strongly limit, direct exchange of gases and contaminants

(dust, microorganisms, etc.) between the culture and the atmosphere. − These devices provide a protected environment for cultivated species, relatively

safe from contamination by other microrganisms, − culture parameters such as pH, oxygen and carbonic dioxide concentration, and

temperature can be better controlled, and provided in known amount. − Moreover, they prevent evaporation and reduce water use, − lower CO2 losses, − permit higher cell concentration, thus reducing operating costs, and attain higher

productivity. Disadvantages, these systems are more expensive to build and operate, due to the need of cooling, strict control of oxygen accumulation, and biofouling, and their use must be limited to the production of very high-value compounds from algae that cannot be cultivated in open ponds.

95

Classification of photobioreactors Photobioreactors can be classified on the basis of both design and mode of operation. In design terms, the main categories of reactors are: (1) flat or tubular; (2) horizontal, inclined, vertical or spiral; (3) serpentine or manifold. An operational classification of PBR would include (4) air or pump mixed and (5) single-phase reactors (filled with media, with gas exchange taking place in a separate gas exchanger), or two-phase reactors (in which both gas and liquid are present and continuous gas mass transfer takes place in the reactor itself). Construction materials provide additional variation and subcategories; for example (6) glass or plastic and (7) rigid or flexible PBR.

Axenic PBR are reactors operated under sterile conditions. Although a major characteristic of PBR is their ability to limit contamination, it must be made clear that an effective barrier, and thus operation under truly sterile conditions, is not achieved except in the few special designs developed expressly for that purpose. I. Tubular photobioreactors 1. Serpentine photobioreactors Serpentine PBR are systems in which several straight transparent tubes are connected in series by U-bends to form a flat loop (the photostage) that can be arranged either vertically or horizontally. Gas exchange and nutrient addition normally take place in a separate vessel. Circulation between the photostage and the gas exchanger is achieved by the use of a pump

Fig. . (a) Serpentine reactors at the Department of Chemical Engineering of the University of Almeria (Spain); (b) A two-plane serpentine reactor at the Centro di Studio dei Microrganismi Autotrofi of the CNR (Florence, Italy).

96

2. Manifold photobioreactors In manifold PBR, a series of parallel tubes are connected at the ends by two anifolds, one for distribution and one for collection of the culture suspension.

4. Helical photobioreactors (bio-coil PBR) Helical PBR consist of small-diameter, generally flexible tubes wound around an upright structure.

97

II. Flat photobioreactors

Fig. . A schematic diagram of the flat plate reactor and its tilt angles.

III. Vertical cylinders and sleeves Units can be consisted of glass columns, 1.8 m in height and 10 cm in diameter. A disposable vertical reactor can be easily built by cutting a suitable length of transparent polyethylene tubing and heat-sealing one end. This bag or sleeve reactor can be suspended from a framework or supported within a mesh frame (the next figure). The culture is mixed by bubbling air from the bottom. Such reactors are used indoors with artificial illumination (generally vertically mounted fluorescent lamps) or outdoors under sunlight.

Fig. . (a) Polyethylene sleeves at the Institute for Applied Research (Beer-Sheva); (b) Annular columns at the Department of Agricultural Biotechnology of the University of Florence (Italy).

98

Polyethylene bag supported within a mesh frame

DESIGN CRITERIA FOR PHOTOBIOREACTORS Design criteria for PBR should aim at achieving high productivities and high efficiency of conversion of light energy, providing, at the same time, the necessary reliability and stability to the cultivation process by means of a cost-effective culture system. An efficient PBR can not be properly designed without adequate knowledge of the physiology in mass culture of the organisms to be cultivated. Since phototrophic microorganisms are highly diverse in their morphology, nutritional and light requirements, and resistance to stresses, PBR can not be designed so as to adapt to all organisms and all conditions. The main design criteria for PBR include: 1. Surface-to-volume ratio (s/v) The ratio between the illuminated surface area of a reactor and its volume (s/v) determines the amount of light that enters the system per unit volume. Generally, the higher the s/v, the higher the cell concentration at which the reactor can be operated and the higher the volumetric productivity of the culture. There is an optimal s/v (or light path) at which maximum productivity per unit of illuminated surface area is obtained. 2. Orientation and inclination Generally, sun-oriented systems (south-facing and tilted so as to intercept maximum solar radiation) achieve higher volumetric productivities. 3. Oxygen accumulation Oxygen concentrations equivalent to four or five times saturation with respect to air, is toxic to many phototrophs, and thus requires frequent degassing. 4. Mixing Mixing is necessary to prevent cells from settling, to avoid thermal stratification, to distribute nutrients, to remove photosynthetically generated oxygen and to ensure that cells experience alternating periods of light and darkness of adequate length.

99

5. Temperature control Maximum productivity can be achieved only at the optimal temperature for growth. PBR generally require cooling at midday. Shading, immersion in a water bath and water spraying are the most common solutions adopted to avoid overheating of PBR outdoors. 6. Supply of carbon dioxide The residence time of the injected CO2 bubbles should be sufficient for complete absorption. 7. Materials Materials for PBR must lack toxicity have high transparency, high mechanical strength, of high durability (resistance to weathering), chemical stability and low cost. Ease of cleaning is also another important operational issue. QUANTITATIVE DETERMINATIONS OF ALGAL DENSITY AND GROWTH

1. Cell count 2. Dry and wet mass 3. Protein concentration determination 4. Chlorophyll determination 5. Total organic carbon (TOC) measurement

100

Mariculture of Seaweeds Introduction Macroscopic marine algae form an important living resource of the oceans. Seaweeds are food important for humans and animals, as well as fertilizers for plants and a source of various chemicals. Seaweeds have been gaining momentum as a new experimental system for biological research and as an integral part of integrated aquaculture systems. We all use seaweed products in our day-to-day life in some way or other. For example, some seaweed polysaccharides are used in toothpaste, soap, shampoo, cosmetics, milk, ice cream, meat, processed food, air freshener, and many other items. In many oriental countries such as Japan, China, Korea, and others, seaweeds are diet staples. Need for Mariculture Traditionally, seaweeds were collected from natural stocks or wild populations. However, these resources were being depleted by overharvesting, so cultivation techniques have been developed. Today, seaweed cultivation techniques are standardized, routine, and economical. Several factors, such as morphology and regeneration capacity of the thallus, as well as complex interaction of irradiance, temperature, nutrients, and water movement, are responsible for the success of large-scale seaweed cultivation. Cultivation methods During the last 50 years, approximately 100 seaweed taxa have been tested in field farms, but only a dozen are being commercially cultivated today. Table 1 provides production data for the top taxa.

TABLE 1 Top cultivated seaweed genera in the world during 2000 (FAO 2003).

Different taxa require different farming methods. Although some seaweeds need one-step farming through vegetative propagation, others need two-step or multistep farming. The latter must be propagated from spores and cannot survive if propagated vegetatively. IN VEGETATIVE CULTIVATION, small pieces of seaweed are taken and placed in an environment that will sustain their growth. When they have grown to a suitable size they are harvested, either by removing the entire plant or by removing most of it but

101

leaving a small piece that will grow again. When the whole plant is removed, small pieces are cut from it and used as seedstock for further cultivation. The seaweed should be held in its environment in several ways (Fig. 1).

FIGURE 1. (a) Rocky substratum with attached seaweed being transplanted to a new site. (b) seaweed attached to rocks with rubber bands; method used for anchoring transplants in soft sediments. (c) Plants inserted with a fork directly into soft sediments. (d) Plants attached to sand-filled plastic tubes. (e) seaweed attached to a rope, which is stretched between two poles pushed into the sediments. (f ) Attachment of plants for rope culture. (g) Bamboo floating frame with seaweed attached to ropes spanning the frame. (h) A floating net with seaweed attached to the meshes.

102

The suitable environment varies among species, but must meet requirements for salinity of the water, nutrients, water movement, water temperature and light.

CULTIVATION INVOLVING A REPRODUCTIVE CYCLE, with alternation of generations, is necessary for many seaweeds; for these, new plants cannot be grown by taking cuttings from mature ones. This is typical for many of the seaweeds.

SEAWEED CULTIVATION IN THE SEA Cultivation occurs along coastal areas. To hold the seaweeds in place, a variety of farm structures are used. These include long lines to which ropes with seaweeds are attached, nets stretched out on frames, and ropes supported by poles. Details of these different systems are provided in the following sections. 1. Long-Line Cultivation Systems In the 1950s, China developed a highly successful method for cultivating Laminaria. In this method, sporelings (“seedlings”) are produced in artificially cooled water at 8-10 C in greenhouses and later planted out in the ocean. For cultivation, Laminaria must go through its life cycle, and this involves an alternation of generations between a large sporophyte - the sporophyte is what is harvested as seaweed- and a microscopic gametophyte. The mature sporophytes form sori -surface organs where sporangia are produced- from which motile zoospores are released. To stimulate zoospore release, a selected parent Laminaria plants are dried for a few hours and placed in the seeding container which is filled with cool seawater. The seed string (a synthetic twine of 2 to 6 mm in diameter or palm line 6 mm in diameter) is placed on the bottom of the same container. Released zoospores are attached to the strings and germinate into male and female gametophytes.

Fig. 2 A Chinese long-line farm for cultivation of Laminaria: The long line is anchored by a rope at each end and held afloat by buoys. Culture lines with attached Laminaria include a spacing segment at the top and bottom of the 2- to 5-m-long rope and weighed. The anchor ropes are held by stakes or concrete weights.

103

As the gametophytes become fertile, they release sperm and eggs that join to form zygotes which attach themselves to the collectors – i.e. the same substrate materials - and develop into seedlings or sporelings. The seedlings are reared into young sporophyte plants 1-2 cm high are then sold to farmers for outplanting in the sea. The strings are then cut into small pieces that are transferred to the sea and inserted into the warp of large diameter, 60 m long culture rope. The ropes with the young sporophytes are kept floating by buoys fixed every 2–3 m. Each end of the rope is anchored to a wooden peg driven into the sea bottom. The ropes with the young sporophytes attached hang down from this rope at 50 cm intervals (Fig. 2). These slowly develop into the large sporophytes that we harvest. The principal difficulties in this kind of cultivation lie in the management of the transitions from spore to gametophyte to embryonic sporophyte; these transitions are usually carried out in land-based facilities with careful control of water temperature, nutrients and light. The Laminaria is harvested in 6-7 months when it is 3-4 metres in length. By the same method, the Japanese also farm a similar kelp, Undaria, which is sold as the food wakame.

FIGURE 3.. (d) Long line with Laminaria after 8 months of growth (Yellow Sea, China). (e) Long line showing attached Laminaria plants (South Korea). (f ) Young sporophytes growing on long line. 2. Net-Style Farm Systems Porphyra, or nori, is the world's most valuable marine crop. The crop is valued at more than 1 billion dollars worldwide and is used mainly for human food. These plants grow mainly in cooler waters. The plants can grow from 5 to 35 cm in length. The thalli are either one or two cells thick, and each cell has one or two chloroplasts with a pyrenoid. Porphyra reproduces by both sexual and asexual modes of reproduction. Its sexual life cycle is heteromorphic and involve both an edible blade phase (gametophytic phase) and a

104

filamentous, microscopic, shell-dwelling, sporophyte called the conchocelis phase. Reproduction cells formed by blades (gametophytic), known as carpospores, colonize shells and grow into small filaments (conchocelis) that generate conchospores. The later can be induced to colonize twine (nets) that is suspended in the sea (see Fig 4), and produce blades, thus completing the life cycle. Blades may also arise from an asexual process involving monospores.

Nori grows as a flat sheet. Porphyra are allowed to grow to 15–30 cm in about 40–50 days before they are harvested (Fig. 5 c,d). The remaining thalli are allowed to grow and may be ready for a second harvest after another 15 to 20 days. Several harvests may be made from the same nets in one growing season. The harvested crop is washed and transferred to an automatic nori-processing machine, which cuts the blades into small pieces. The nori is then processed by the cultivator into dried rectangular sheets or processed by the manufacturer per market requirements.

Fig. 4 A Japanese Porphyra culture net system: Poles hold the net in place so that it is exposed at low tides. The Porphyra grows attached to the nets.

105

3. Line and Rope Farm Systems Farmers in the Philippines use rope and lines to grow tropical seaweeds. These seaweeds comprise species of genera Eucheuma and Kappaphycus. Plants are propagated vegetatively, the seaweeds are tied to the lines, and the lines are then staked over the bottom. The water level should be 0.5 to 1.0 meter during low tide and not more than 2.0 to 3.0 m during high tide. The lines are constructed to form plots or units of a standard size (Fig. 6c). Seedlings weighing between 50 and 100 g are tied to the monolines at 25- to 30-cm intervals using soft plastic tying material called tie-tie. Usually the plants are harvested after 45 days when each seedling weighs up to 1 kg (Fig. 6e). The best looking healthy plants are selected to serve as seedlings for the next crop. The remaining plants are sun dried or sold fresh in the market. Eucheuma and Kappaphycus are important carrageenophytes (80% of world’s carrageenan production).

FIGURE 6. (a) Rope cultivation of Gracilaria using monofilament long lines. (b) Enlarged image showing a Gracilaria plant held within the twists of the lone line rope. (c) Eucheuma farmers harvesting plants from submerged long lines. (d) Open water cultivation and harvesting of Kappaphycus; diver bringing a large plant to the boat. Eucheuma and Kappaphycus are tied to the lines that are held just above the sediment surface. The depth of the plants are adjusted so that they are not exposed at low tides. (e) Typical outrigger boat used for open water harvesting.

106

4. Offshore or Deep-Water Seaweed Cultivation Various attempts were made to cultivate the brown alga Macrocystis pyrifera on farm structures designed for use in deep water. The nutrients for these seaweeds were to come from cold, deep waters that would be pumped up into the growing kelps. The benefits of this approach is that growth of macroalgae would not be constrained by available shallow nearshore regions. Despite several trials using different farm designs, operational problems prevented the production of actual kelp crops. However, the experiments did establish that M. pyrifera could grow in an open ocean environment, and that deep waters supplied ample nutrients for sustained growth without toxic side effects. It is probable that these research results could be extended to other brown kelps, such as Laminaria spp. or Undaria spp. However, no reports are available that describe such offshore-farming approaches with green or red algae. LAND-BASED CULTIVATION SYSTEMS TANKS These systems generally use seaweeds growing in tanks receiving a steady stream of aeration and seawater. The aeration provides vigorous water movement in the tanks, sending the algal thalli up and down in the water column in a circular pattern. This vigorous aeration permits rapid uptake of dissolved carbon dioxide, and bringing the biomass to the surface into the light. The use of tanks may provide the greatest productivity per unit area per day and is more efficient than any other type of farming. Efficiency of these systems is very much dependent on the input of various types of energy (compressed air for bubbling, CO2, and pumping water) and nutrients. Carbon supply can be improved by either pumping more seawater or by adding CO2. The temperature and salinity also can be manipulated by pumping more seawater. The pH of the tanks should be managed in the range of 7.9 to 8.3, and the nutrient status of the medium must be monitored. Tanks should be cleaned regularly and epiphytes must be controlled. Tank systems also may hold promise for the processing of polluted water for specific products, the removal of extra nutrients from wastewater, or for energy production.

PONDS Macroalgae can also be grown in ponds. An advantage of this approach is the low-operating costs. Generally, water exchange in the ponds is accomplished by use of tide gates. Seaweed yields are low because of the lack of water movement in the ponds and the low exchanges of water.

Tank systems are usually in smaller modules that allow a predictable maintenance schedule, several steps however, can be precisely controlled and managed to reduce the labor input, although this type of system has high operational costs. Ponds are larger, and a significant outbreak of epiphytes or other weedy species may be much harder to bring under control.

107

POPULATION DYNAMICS