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Transcript of PhD Thesis_Chad A. Keyser
U N I V E R S I T Y O F C O P E N H A G E N U N I V E R S I T Y O F C O P E N H A G E N
PhD thesis
Chad Alton Keyser
Protecting plants against pests and pathogens with
entomopathogenic fungi: The biocontrol agent Metarhizium, its distribution, application, and interaction with other
beneficial fungi
Academic Advisor: Nicolai Vitt Meyling
Submitted: 30 January, 2015
This thesis has been submitted to the PhD School of The Faculty of Science, University of Copenhagen
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Institution: University of Copenhagen, Faculty of Science
Department: Department of Plant and Environmental Sciences (PLEN)
Author: Chad Alton Keyser
Title: Protecting plants against pests and pathogens with entomopathogenic fungi:
the biocontrol agent Metarhizium, its distribution, application, and interaction
with other beneficial fungi.
Academic advisor: Nicolai Vitt Meyling
Co-advisor: Kristian Thorup-Kristensen
Submitted: 30 January 2015
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Acknowledgments
“It is only with the heart that one can see clearly, for the most essential things are invisible to the eye."
― Hans Christian Andersen, The Ugly Duckling
Through this acknowledgment I would like to express my profound appreciation to the many
individuals that have supported and encouraged me during the course of my PhD program. Throughout the
last three years I have grown significantly as a scientist and as a person – this growth is due mainly to the
collaborations, friendships and nurturing influence of the many people I have had the opportunity to interact
with.
I first met Nicolai Meyling in 2009 at a scientific conference in Park City, Utah, as we stood in a
crowded hall waiting for seating to begin. During our short conversation I was impressed by his attentive
interest as I explained what I was working on as a Masters student. As my supervisor, Nicolai has continued
to support and facilitate my efforts and growth. He has patiently steered my ideas in scientifically-relevant
directions and ensured that my project was progressing. I am very grateful to Nicolai for his relaxed manner,
thoughtful comments and suggestions, and the diligence and effort he has put into mentoring me.
The Section for Organismal Biology (SOBI) has assembled an exemplary team of insect
pathologists. It has been a pleasure to work alongside such a cohesive group, to share ideas, experience and
encouragement – my experience here will always serve as a paragon for future collaborations. As the head
of this research group, I am grateful to Jørgen Eilenberg for his infectious enthusiasm, his example of
efficiency and his effort to make me feel part of the team. Also, I am very grateful to Bernhardt Steinwender
for both his friendship and constant willingness to listen and discuss even the most ridiculous of ideas. I am
also thankful to Henrik de Fine Licht for his patients in instructing me in art of AFLP analysis. The Team
consists of many more PhD fellows, post-docs and professors who have each individually encouraged,
inspired, taught and helped me in many ways and for which I am truly appreciative.
It has been a great pleasure to work alongside many skilled technicians and assistants. I am
especially grateful to Louise Munk Larsen for her ample technical skills and continued willingness to drop
what she is doing to help. I thank Sylvia Mathiasen and Vinnie Deichmann for their assistance with my
molecular work. I am also grateful to Line Lykke, Lærke Thordsen, Martina Falagiarda, Jesper Anderson,
Azmi Mahmood, Darren Thomsen and the many other student helpers that have assisted me in many aspects
of my experiments – I would not have been able to accomplish what I have needed to do without their
diligent effort and skills.
I have also been fortunate to have Kristian Thorup-Kristensen as a co-advisor. I am thankful to him
for sharing his expertise in working with plants and in experimental design, as well as including me as part
of his team. I also thank Birgit Jensen for her assistance in working with Fusarium and Clonostachys and her
interest and willingness to train and assist me throughout the study for the second Manuscript.
Living in Denmark and attending the University of Copenhagen has been the experience of a
lifetime. I am thankful to Plant Biosystems Elite Environment at the University of Copenhagen for funding
my PhD research. I am also grateful to the Department of Plant and Environmental Sciences and the Section
for Organismal Biology for hosting and providing necessary facilities for my studies.
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I am also supremely grateful for the support and encouragement I have received from my families. I
recognize that living overseas has been difficult for both my family and my wife’s family; I sincerely
appreciate their willingness to accept my decision to pursue this degree and the support and love they have
shown which has been an enabling power to finish. I also appreciate the family and friends that have found
the opportunity to visit us and share in this experience – their refreshing visits have made the distance more
bearable.
Most importantly, I would like to express sincere gratitude to my beautiful wife Shannon and three
energetic children: Myra, Alexys and Noah. They willingly left behind their friends, families, job and
comforts to follow me on an unknown path. My children have worked hard, learned the difficult language
and adjusted quickly to the Danish lifestyle – their adaptability and bravery has given me strength. Shannon
has also thrived and grown to love European living – her infectious eagerness to explore and discover the
world around us has lifted and strengthened our whole family. I could not have succeeded in completing this
program if not for her. Having my best friend by my side and knowing that she supports my ambitions has
made this experience truly enjoyable. It is to my wife and children I dedicate this work and my life.
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TABLE OF CONTENTS
ACKNOWLEDGMENTS ....................................................................................................................................... 3
I. LIST OF INCLUDED MANUSCRIPTS ........................................................................................................... 6
II. SUMMARY .................................................................................................................................................. 7
III. DANSK RESUMÈ ......................................................................................................................................... 9
IV. THESIS OBJECTIVES ................................................................................................................................ 11
1. INTRODUCTION ........................................................................................................................................... 12
2. THE ENTOMOPATHOGENIC FUNGAL GENUS METARHIZIUM ................................................................... 13
2.1 Phylogeny and Taxonomy ..................................................................................................................... 15
2.2 Ecology .................................................................................................................................................. 18
2.2.1 Abundance and distribution ............................................................................................................ 18
2.2.2. Abiotic factors that affect survival and growth ............................................................................. 21
2.2.3 Environmental dissemination pathways ......................................................................................... 22
3. TROPHIC INTERACTION .............................................................................................................................. 23
3.1 Metarhizium ↔ Insects .......................................................................................................................... 24
3.2 Metarhizium ↔ Plants ........................................................................................................................... 26
3.3 Metarhizium ↔ Other microorganisms ................................................................................................. 29
3.4 Multi-trophic interactions with Metarhizium ........................................................................................ 31
3.4.1 Metarhizium ↔ Other microorganisms ↔ Insects ......................................................................... 31
3.4.2 Metarhizium ↔ Other microorganisms ↔ Plants .......................................................................... 32
3.4.3 Metarhizium ↔ Plants ↔ Insects ................................................................................................... 32
3.4.4 Metarhizium ↔ Other microorganisms ↔ Plants ↔ Insects ......................................................... 33
4. METHODOLOGY ......................................................................................................................................... 34
4.1 Selective media ...................................................................................................................................... 34
4.2 Bioassay statistics .................................................................................................................................. 37
4.2.1 Experimental design ....................................................................................................................... 37
4.2.2 Types of Statistical Analyses .......................................................................................................... 38
V. CONCLUSION AND FUTURE PERSPECTIVES .............................................................................................. 42
VI. REFERENCES ............................................................................................................................................ 44
VII. APPENDIX ................................................................................................................................................ 52
Manuscript 1 ................................................................................................................................................ 52
Manuscript 2 ................................................................................................................................................ 63
Manuscript 3 ................................................................................................................................................ 90
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i. List of included Manuscripts
Manuscript 1
METARHIZIUM SEED TREATMENT MEDIATES FUNGAL DISPERSAL VIA ROOTS AND INDUCES
INFECTIONS IN INSECTS
Chad A. Keyser, Kristian Thorup-Kristensen, & Nicolai V. Meyling
Status: Published in Fungal Ecology, October 2014, Vol. 11, pg. 122-131
License Number: 3531750730534
Manuscript 2
BEST OF BOTH WORLDS: DUAL EFFECTS OF METARHIZIUM SPP. AND CLONOSTACHYS ROSEA
AGAINST AN INSECT AND A SEED-BORNE PATHOGEN IN WHEAT
Chad A. Keyser, Birgit Jensen & Nicolai V. Meyling
Status: Under Review - Pest Management Science, submitted 22 Dec, 2014
Manuscript 3
DIVERSITY OF METARHIZIUM FLAVOVIRIDE POPULATIONS ASSOCIATED WITH ROOTS OF CROPS IN
DENMARK
Chad A. Keyser, Henrik H. de Fine Licht, Bernhardt M. Steinwender & Nicolai V. Meyling
Status: Manuscript
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ii. Summary
Background: Insect-pest management is an increasingly important area of research. Efforts
to maximize agricultural output are significantly dependent on reliable means for pest suppression.
Biological control, or the use of living organisms to suppress a pest population, is among one of the
leading alternatives to traditional chemical-based pesticides for crop protection. For the past 130
years several isolates of the fungal genus Metarhizium has been lead candidates among potential
fungal-based biological control agents (BCAs) for insect pest control in agriculture. However, the
majority of Metarhizium research has emphasized product development and application, largely
neglecting the ecological and fundamental aspects. Inconsistent field reliability and economic
viability have limited wider implementation of many BCAs, including Metarhizium-based products;
an increased understanding of the fundamental ecology and environmental interactions has
substantial potential to improve biological control efforts.
The overall aim of this thesis was to improve the current understanding of how members of
the fungal genus Metarhizium naturally occur in association with roots of crops in Denmark and
interact with other organisms in relation to plant roots when applied as BCAs. Several scientific
studies were conducted to answer important ecological questions regarding Metarhizium spp.
interactions and their use as BCAs. The results of these studies are presented in three manuscripts.
Manuscript 1: Recent research has revealed that many Metarhizium spp. interact with plants
in the rhizosphere and have been shown to increase nutrient uptake and promote plant growth. In
Manuscript 1 we investigate how might the fungus benefit from a plant association; namely,
whether the plant provides a means of dispersal for the otherwise immobile fungus; as well as if the
fungus maintains pathogenicity to insects while interacting with the plant. We found that when
Metarhizium spp. were inoculated as conidia on wheat seeds they were able to disperse through the
soil with the growing root and be re-isolated from lower portions of the root. Furthermore we
observed that when washed roots were placed with Tenebrio molitor larvae, the larvae would
succumb to Metarhizium spp. infection.
Manuscript 2: Agricultural yields are threatened by multiple pests including insects and
plant pathogens. Often the control of these pests requires the application of multiple biological
control agents. In Manuscript 2 we investigate whether the mycoparasite Clonostachys rosea,
commonly used to control plant-fungal pathogens, can be applied jointly with Metarhizium spp. to
control both a plant pathogen and an insect pest. In this study we observed that C. rosea was highly
efficacious at controlling Fusarium culmorum alone and in combination with Metarhizium – when
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applied as a conidial seed treatment to wheat seeds. Additionally, we observed that while a
significant level of T. molitor were infected with Metarhizium spp. after a combined treatment,
there was a slight reduction in virulence when either C. rosea or F. culmorum were also present
when compared to Metarhizium spp. only seed treatments. Based on the result of the direct
inoculation bioassay of T. molitor larvae in which we did not observe a reduction in virulence when
comparing combination treatments to individual treatments, we suspect that the virulence reduction
is the result of resource competition on the growing root and not direct mycoparasitism.
Manuscript 3: An awareness of the composition and distribution of naturally occurring
Metarhizium spp. communities is important to understanding their role to insect host regulation.
However there is an acute lack of ecological studies that assess the occurrence and community
structure of entomopathogenic fungi. The objective of Manuscript 3 was to evaluate the
occurrence, diversity and community structure of Metarhizium spp. isolates obtained from different
crops at geographically separated agricultural fields in Denmark. Root and root-associated soil was
sampled from wheat, oilseed rape, and bordering uncultivated grass fields at three different
locations; 132 new Metarhizium isolates were obtained. Morphological data and sequencing of the
rDNA intergenic spacer region (IGS) revealed that 118 of the isolates belonged to Metarhizium
flavoviride, 13 M. brunneum and one M. majus. We then further characterized the intraspecific
variability within M. flavoviride by unspecific markers (i.e., AFLP identification) to evaluate
diversity and potential crop and/or area associations. We found there was a high level of diversity
among the M. flavoviride isolates indicating that the isolates were not of the same clonal origin,
however due to insufficient loci in the AFLP analysis we were not able to determine haplotype
groupings or confirm any habitat associations. We suggest that the development of more specific
markers would greatly improve our ability to evaluate M. flavoviride diversity. This represents the
first time that an in-depth analysis of the molecular diversity within a large isolate collection of the
species M. flavoviride has been reported.
Overall the scientific studies presented in this thesis are both important and novel to the field
of Metarhizium research; these studies advance the current knowledge of the ecological significance
of Metarhizium spp. as a naturally occurring microorganism and increase our understanding of their
interactions as biological control agents with other organisms. Furthermore, this thesis presents the
background literature and motivation for the research and their implication to the field of insect
pathology.
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iii. Dansk resumè
Baggrund: Bekæmpelse af skadedyr er et vigtigt forskningsområde. Mulighederne for at øge
landbrugsudbyttet er afhængigt af pålidelige bekæmpelsesmetoder. Biologisk bekæmpelse, brugen
af levende organismer til at begrænse skadedyrspopulationer, er en af de væsentligste alternativer til
kemisk baseret plantebeskyttelse. I løbet af de seneste 130 år har flere isolater af den insektpatogene
svampeslægt Metarhizium blevet førende kandidater til svampebaseret biologisk bekæmpelse af
skadedyr. Dog har hovedparten af forskning i Metarhizium fokuseret på produktudvikling og
udbringning, hvor forståelse af grundlæggende økologiske aspekter har blevet negligeret.
Varierende pålidelighed har begrænset implementeringen af mange biologiske
bekæmpelsesprodukter, inklusiv flere baseret på Metarhizium. En øget forståelse af de
fundamentale økologiske og miljømæssige interaktioner, hvori Metarhizium indgår, har stort
potentiale til at forbedre brugen af biologisk bekæmpelse.
Det overordnede formål med denne afhandling var at øge forståelsen af hvordan medlemmer
af svampslægten Metarhizium indgår i naturlig associering med rødder af afgrøder i Danmark og
hvordan de interagerer med andre organismer i relation til planterødder når de tilføres ved biologisk
bekæmpelse. Flere videnskabelige studier blev gennemført for at svare på dette, og resultaterne er
præsenteret i tre manuskripter.
Manuskript 1: Det er for nyligt blevet videnskabeligt vist at flere arter af Metarhizium
interagerer med planter i rhizosfæren og at dette kan øge næringsstofoptag og vækst hos planten. I
Manuskript 1 undersøges det om svampen kan have fordel af denne interaktion ved at bruge
plantens rødder til transport i jorden, og om svampen bevarer sin evne til at inficere insekter ved at
interagere med planten. Det blev fundet, at når Metarhizium spp. blev inokuleret som konidier på
frø af hvede, kunne svampen sprede sig gennem jord med de voksende rødder og blive genisoleret
fra den nedre del af rødderne. Desuden var vaskede rødder infektive mod larver af melorme
Tenebrio molitor, som efter inkubering sammen med rødder døde af Metarhizium infektion.
Manuskript 2: Afgrøder bliver ofte angrebet af flere organismer, primært insekter og
plantepatogener, hvilket kræver samtidig brug af flere biologiske bekæmpelsesmidler. I Manuskript
2 blev det undersøgt, om nyttesvampen Clonostachys rosea, som normalt bruges til at bekæmpe
plantepatogener, kan blive anvendt sammen med Metarhizium spp. til at bekæmpe både insekter og
plantesygdomme på samme tid. Det blev observeret at C. rosea var meget effektiv til at bekæmpe
Fusarium culmorum alene og sammen med Metarhizium spp., når de to typer af svampe blev tilført
som konidier på frø af hvede. Desuden blev larver af melorme inficeret af Metarhizium spp. både
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når denne svamp blev tilført alene og sammen med C. rosea eller F. culmorum, men infektionen var
en smule nedsat i kombinationerne. Ved direkte inokulering af larverne med sammen
svampekombinationer sås ikke denne reduktion. Reduktionen observeret ved planteinokuleringen
kunne derfor skyldes en indirekte interaktion på planteroden og ikke direkte interaktion som
mykoparasitisme mellem svampene.
Manuskript 3: Det er afgørende af kende til den naturlige forekomst og udbredelse af
Metarhizium spp. for at forstå deres bidrag til regulering af insektpopulationer. Der findes dog
fortsat kun få studier af den naturlige forekomst af insektpatogene svampe. Formålet med studiet
præsenteret i det tredje manuskript var at beskrive forekomst, udbredelse og diversitet af
Metarhizium spp. i forbindelse med rødder af forskellige afgrøder i Danmark på tre geografisk
afgrænsede lokaliteter. Rødder og rod-associeret jord blev indsamlet på hver lokalitet fra
vinterhvede, raps, og fra et uforstyrret græsningsareal. 132 Metarhizium isolater blev indsamlet.
Morfologisk og DNA sekventering viste, at 118 af isolaterne tilhørte arten Metarhizium flavoviride,
13 var M. brunneum, og et var M. majus. Ved yderligere karakterisering af intraspecifik variation i
M. flavoviride med uspecifikke markører (AFLP) blev diversitet og potentiel lokalitet- eller
afgrødespecificitet undersøgt. En høj grad af diversitet blev fundet med de anvendte markører,
hvilket indikerer at de ikke alle har samme klonale ophav, men metoden var ikke tilstrækkelig til at
identificere lokalitet- eller afgrødespecificitet. Specifikke markører udviklet til M. flavoviride vil
være nødvendige for at undersøge dette. Dette studie er det første hvor arten M. flavoviride blev
undersøgt mht. molekylær diversitet ved brug af en større samling af isolater.
De videnskabelige studier præsenteret i denne afhandling er både vigtige og nye indenfor
forskningen i Metarhizium. Studierne øger den nuværende viden om økologisk betydning af
Metarhizium spp. som naturlig forekommende mikroorganisme samt ved interaktioner med planter
og med andre mikroorganismer. Desuden giver denne afhandling en gennemgang af litteraturen om
emnet og betydningen af den præsenterede forskning for insektpatologi.
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iv. Thesis Objectives
The aim of this thesis is to advance our understanding of how members of the entomopathogenic
fungal genus Metarhizium interact with other organisms, with an emphasis placed on its role as a
biological control agent. To accomplish this goal the following research questions were
investigated:
■ Can plant roots act as a vehicle to disseminate Metarhizium in soil? Additionally, while
associating with plants, do Metarhizium spp. maintain their pathogenicity to insects?
■ In a seed-treatment biocontrol context, what interactions occur between other organisms,
namely: the mycoparasitic fungus Clonostachys rosea, and the plant pathogenic fungus
Fusarium culmorum?
■ What is the prominence and species composition of naturally occurring Metarhizium in roots
and soil within different agro-ecosystems in Sjælland, Denmark?
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1. Introduction
Agricultural production is incalculably important to human existence both from an
economical as well as a nutrient-resources perspective. Worldwide estimates suggest that currently
38% of the Earth’s terrestrial surface is dedicated to agricultural endeavors (Foley et al., 2011).
Furthermore, it has been projected that from 2005 to 2050 global crop production will need to
increase as much as 110% to meet the caloric and protein demands of the world population (Tilman
et al., 2011). We cannot expect to meet the growing agricultural needs by merely dedicating more
land to food production; increasing the productivity of the current agricultural systems is vital to our
future (Tilman et al., 2011). A significant limiting factor to agriculture yields are pests – this
includes herbivores (e.g., arthropods), weeds and plant pathogens. Over the last century advances
in chemical pesticide development have greatly mitigated pest related crop losses. However, due to
pesticide resistance and an increased awareness of deleterious effects on non-target organisms,
including humans, reliable alternative methods for controlling pests are desperately needed.
Biological control is an important alternative which has potential to effectively control pest
populations with limited risk (Hajek, 2004).
Biological control can be defined as “the use of living organisms to suppress the population
of a specific pest organism, making it less abundant or less damaging then it would otherwise be”
(Eilenberg et al., 2001). There are several types of organisms that have been identified as biological
Glossary of Terms
Agroecosystem Agricultural ecosystem - Specialized ecosystem which has been manipulated by human activities with the aim to produce high levels of organic output. Includes living and non-living components and their interactions.
Anamorph The asexual (conidial or imperfect) stage in the life history of a fungus.
BCA Biological control agent – the organism used for Biological control
Bioassay The measurement of the potency of any BCA, by means of the response which it produces in a living host.
Biological control The use of living organisms to control (usually meaning to suppress) undesirable animals and plants.
Entomopathogen A microbe affecting insects (or in a more general sense, other terrestrial arthropods including arachnids), usually causing mortality in the host (as opposed to a more benign relationship).
Fungal endophyte An asymptomatic plant-colonizing fungus that lives a portion of its life cycle inside the plant.
Pathogenicity The quality or state of being pathogenic. The potential ability to produce disease. Pathogenicity is qualitative, an all-or-none concept
Rhizosphere The narrow region around the plant root that is directly influenced by root secretions and associated soil microorganisms.
Teleomorph The sexual stage in the life history of a fungus.
Virulence The disease-producing power of a microorganism. Virulence can be quantified.
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control agents (BCAs), including: predators, parasitoids, parasitic nematodes, bacteria, viruses,
fungi and microsporidia (Hajek, 2004), the latter group is now recognized and a basal fungal group
(James et al., 2006). Each BCA has different characteristics which determine their effectiveness in
a particular circumstance. Understanding the environmental factors that contribute to effectiveness
will largely determine the success of a BCA. For many years research regarding the fundamental
ecology of these organisms has had far less priority than product development; this has likely led to
inconsistent results in the field (Vega, 2008). The present thesis contributes in part, to increasing
our understanding of the complex interactions involved between a particular fungal BCA and other
important organisms in its environment, within a biological control context.
2. The entomopathogenic fungal genus Metarhizium
Entomopathogenic fungi are fungal organisms that have the ability to infect and cause
disease in an arthropod. The kingdom Fungi is estimated to contain more than 5.1 million species
(O'Brien et al., 2005), of those, 750-1000 species are pathogenic to insects (Vega et al., 2012).
Fungi of the Ascomycota genus Metarhizium (Hypocreales: Clavicipitaceae) are among one
of the most studied groups of entomopathogenic fungi, in fact in the last decade the number of peer-
reviewed publications has increased substantially (Figure 1). Metarhizium spp. are ubiquitously
found in terrestrial ecosystems worldwide, having been isolated from every continent except
Antarctica (Roberts and St. Leger, 2004). Many species of Metarhizium have a wide host range,
like M. brunneum and M. robertsii, infecting at least seven insect orders (Veen, 1968;
Zimmermann, 1993); however a few species are known to be host specific like M. acridum which
only infects some taxa in the order Orthoptera (Driver et al., 2000; Wang et al., 2011). In addition
to their host range there are several other key attributes that make Metarhizium spp. ideal candidates
for BCAs, including: the infection process is topical (does not need to be ingested by host),
infectious conidia can be mass produced on artificial media, remain viable and can be easily
0
300
600
900
1200
1500
1975-1979 1980-1984 1985-1989 1990-1994 1995-1999 2000-2004 2005-2009 2010-2014
Nu
mb
er
of
Pu
blicati
on
s
Figure 1. The number of peer-reviewed publications published of 5 year periods for the last 40 years according to a search on web of science with the key word “Metarhizium”.
14
disseminated, and many species of Metarhizium produce secondary metabolites known as
destruxins which are toxic to invertebrates and help the pathogen overcome the host immunity
quickly (Dorta et al., 1996; Zimmermann, 2007).
The infection process of Metarhizium spp. to a suitable host was reviewed by Zimmermann
(2007) and is summarized in Figure 2. He describes the process in 6 steps including: 1. Attachment,
in which the conidia adheres to the cuticle using a combination of hydrophobic interaction and
specialized adhesion proteins; 2. Germination and appressoria formation; 3. Penetration through the
cuticle, which is mechanical but aided by the production of enzymes including proteases, chitinases
and lipases; 4. Overcoming host defenses, often by the production of novel destruxins; 5.
Proliferation within the host, generally via the production of blastospores or hyphae; and lastly, 6.
Outgrowth and production of new infective conidia.
Figure 2: The infection process, an illustration showing the 6 stages of fungal infection in an insect: 1. Attachment; 2. Germination and appressoria formation; 3. Penetration through the cuticle; 4. Overcoming host defenses; 5. Proliferation within the host; 6. Outgrowth and production of new infective conidia. Illustration by C. A. Keyser.
15
2.1 Phylogeny and Taxonomy
The taxonomy of the Genus Metarhizium (Family: Clavicipitaceae, Order: Hypocreales,
Class: Sordariomycetes Phylum: Ascomycota, Kingdom: Fungi) has been revised many times over
the years. In 1883 Russian mycologist Sorokin first introduced the name Metarhizium as the genus
name for fungi that are the causal agent of insect disease “green muscardine”, which had originally
been called Entomophthora anisopliae by Elia Metchnikoff in 1879 (Zimmermann et al., 1995).
For the last 130 years the genus name Metarhizium has persisted, however many of the species
names belonging to this genus have changed.
Many fungi are pleomorphic, i.e., they have different life stages which are morphologically
distinct – often the different stages have been identified as different organisms. To help standardize
the descriptions the term teleomorph is used to describe the sexual stage, anamorph to describe the
asexual stage, and holomorph when both are present (Hennebert and Weresub, 1977). Species of
the genus Metarhizium have historically been considered anamorphic fungi (i.e., only exhibiting the
asexual stage and reproduce clonally by mitosporic conidia production) and placed in the former-
division Deuteromycota; however the discovery of a sexual and asexual stage (Liang et al., 1991),
as well as molecular analysis have facilitated their placement in the phylum Ascomycota (Kepler et
al., 2014). In this thesis only the anamorphic stage of Metarhizium is discussed.
Another challenge for Metarhizium taxonomy is that many species of Metarhizium are
morphologically similar, so identification based on morphological attributes is difficult. Tulloch
(1976) made a major revision of the genus Metarhizium based on drawings and the morphological
descriptions available, she reduced all known taxa to two speices, M. flavoviride and M. anisopliae.
The next major revision of the genus was performed by Driver et al. (2000) using ITS sequence data
for phylogenetic analyses; they observed a high level of genetic diversity and were able to identify
ten distinct clades, however they restricted their descriptions to varieties rather than species due to
limited resolution and support in the sequence analysis. Bischoff et al. (2009) used a multigene
phylogenetic approach to resolve the M. anisopliae group which at the time consisted of 4 varieties
as defined by Driver et al. (2000); i.e., M. anisopliae var. acridum, M. anisopliae var. anisopliae,
M. anisopliae var. lepidiotae, and M. anisopliae var. majus. They describe ten species within the
M. anisopliae complex (viz., M. anisopliae, M. acridum, M. brunneum, M. globosum, M.
guizhouense, M. lepidiotae, M. majus, M. pingshaense, and M. robertsii) (Bischoff et al., 2009).
The taxonomic clarification of the Metarhizium genus was continued by Kepler et al. (2014) and the
M. flavoviride complex was resolved into four species (viz., M. flavoviride, M. koreanum, M.
16
minus, and M. pemphigi). Additionally, in this revision an effort was made to reevaluate fungal
nomenclature with the intention to give one name to one fungus, regardless of life stage (Taylor,
2011). In doing this Kepler et al. (2014) transferred many taxa from Chamaeleomyces,
Metacordyceps and Nomuraea to Metarhizium. The genus Metarhizium now includes 36 species
(Table 1). Isolates described as “M. anisopliae” or “M. flavoviride” in studies published prior to
(and sometimes after) the 2009 and 2014 taxonomic revisions are now designated as “M. anisopliae
sensu lato” (s.l.) or “M. flavoviride s.l.” if the new taxonomic identity according to Bischoff et al.
(2009) or Kepler et al. (2014) is unknown or not specified, M. anisopliae and M. flavoviride
identified using the current taxonomic criteria are labeled using the sensu stricto (s.s.) designation.
As noted by Steinwender (2013) “taxonomy is not set in stone but rather a snapshot of a given
moment”, it is likely the genus Metarhizium will continue to develop and change as our
understanding of the complexity of life improves.
17
Table 1: Current Species of the Genus Metarhizium, the authorities and year of description – arranged alphabetically.
Species name Authorities, year of description
M. acridum (Driver & Milner) J.F. Bisch., S.A. Rehner & Humber, 2009
M. album Petch, 1931
M. anisopliae (Metsch.) Sorokin, 1883
M. atrovirens (Kobayasi & Shimizu) Kepler, S.A. Rehner & Humber, 2014
M. brasiliense Kepler, S.A. Rehner & Humber, 2014
M. brittlebankisoides (Zuo Y. Liu, Z.Q. Liang, Whalley, Y.J. Yao & A.Y. Liu) Kepler, S.A. Rehner & Humber, 2014
M. brunneum Petch, 1935
M. campsosterni (W.M. Zhang & T.H. Li) Kepler, S.A. Rehner & Humber, 2014
M. carneum (Duché & R. Heim) Kepler, S.A. Rehner & Humber, 2014
M. flavoviride W. Gams & Rozypal, 1973
M. frigidum (Driver & Milner) J.F. Bisch. & S.A. Rehner, 2006
M. globosum J.F. Bisch., S.A. Rehner & Humber, 2009
M. granulomatis (Sigler) Kepler, S.A. Rehner & Humber, 2014
M. guizhouense Q.T. Chen & H.L. Guo, 1986
M. guniujiangense (C.R. Li, B. Huang, M.Z. Fan & Z.Z. Li) Kepler, S.A. Rehner & Humber, 2014
M. indigoticum (Kobayasi & Shimizu) Kepler, S.A. Rehner & Humber, 2014
M. khaoyaiense (Hywel-Jones) Kepler, S.A. Rehner & Humber, 2014
M. koreanum Kepler, S.A. Rehner & Humber, 2014
M. kusanagiense (Kobayasi & Shimizu) Kepler, S.A. Rehner & Humber, 2014
M. lepidiotae (Driver & Milner) J.F. Bisch., S.A. Rehner & Humber, 2009
M. majus (J.R. Johnst.) J.F. Bisch., S.A. Rehner & Humber, 2009
M. marquandii (Massee) Kepler, S.A. Rehner & Humber, 2014
M. martiale (Speg.) Kepler, S.A. Rehner & Humber, 2014
M. minus (Rombach, Humber & D.W. Roberts) Kepler, S.A. Rehner & Humber, 2014
M. novozealandicum Kepler, S.A. Rehner & Humber, 2014
M. owariense (Kobayasi) Kepler, S.A. Rehner & Humber, 2014
M. owariense f. viridescens (Uchiy. & Udagawa) Kepler, S.A. Rehner & Humber, 2014
M. pemphigi (Driver & R.J. Milner) Kepler, S.A. Rehner & Humber, 2014
M. pingshaense Q.T. Chen & H.L. Guo, 1986
M. pseudoatrovirens (Kobayasi & Shimizu) Kepler, S.A. Rehner & Humber, 2014
M. taii Z.Q. Liang & A.Y. Liu, 1991
M. rileyi (Farl.) Kepler, S.A. Rehner & Humber, 2014
M. robertsii J.F. Bisch., S.A. Rehner & Humber, 2009
M. viride (Segretain, Fromentin, Destombes, Brygoo & Dodin ex Samson) Kepler, S.A. Rehner & Humber, 2014
M. viridulum (Tzean, L.S. Hsieh, J.L. Chen & W.J. Wu) B. Huang & Z.Z. Li, 2004
M. yongmunense (G.H. Sung, J.M. Sung & Spatafora) Kepler, S.A. Rehner & Humber, 2014
18
2.2 Ecology
Despite having more than 100 years’ worth of research interest, we are only beginning to
understand the ecology of Metarhizium spp. and the important role they play in the ecosystem.
There are two main reasons why the natural ecology of Metarhizium is important to biological
control: first, as a ubiquitous organism infectious to insects, understanding the natural occurrence
and distribution, and the contributions of Metarhizium in regulating insect populations is highly
relevant; and second, understanding how Metarhizium interacts with other organisms and is affected
by abiotic factors will help optimize how to most effectively use them as BCAs.
Bruck (2010) pointed out that in plant pathology a concept known as the “disease triangle”
is often used to describe the interaction between a host, a pathogen, and the environment; he
suggested that this same concept should also be applied to biological control. By emphasizing a
total ecological approach to Metarhizium spp. research, which focuses on both the direct and
indirect effects of biotic and abiotic factors in the environment, we gain greater clarity of the role
Metarhizium spp. play in the ecosystem. In this section I will discuss with regard to Metarhizium:
2.2.1. Abundance and distribution; 2.2.2. Abiotic factors that affect survival and growth; and 2.2.3.
Environmental dissemination pathways. In section 3 (below) I will discuss biotic interaction that
occur between Metarhizium and other organisms.
2.2.1 Abundance and distribution
The United States Department of Agriculture’s (USDA) Agricultural Research Service
Collection of Entomopathogenic Fungal Cultures (ARSEF), Ithaca, NY, hosts one of the largest
libraries of entomopathogenic fungal isolates collected from all over the world. This collection has
over 1500 different isolates of Metarhizium, however most of these isolates, as well as the many
others that have been collected over the years, were collected not with the intention to understand
abundance and distribution but rather to find new potential products for commercialization:
examples include the LUBILOSA project (Roberts and St. Leger, 2004), in which researchers
scoured the African and Australian continents searching for entomopathogenic fungi with the intent
to develop a BCA for locust control. More recently, an 8 year USDA-APHIS project which
surveyed 30,000 soil samples in the western US and collected more than 2,000 new isolates of
Metarhizium with a goal to find M. acridum in USA soil (C. A. Keyser, unpublished data). While
these “goal-orientated” types of surveys often produce useful information about the ecology and
distribution of Metarhizium in nature; they are not designed as ecological studies and so many of
the conclusions they can provide are incomplete.
19
There have, however, been several studies intended to investigate Metarhizium occurrence
in both natural habitats and agroecosystems (Table 2); it is noteworthy that there are a lack of
studies from latitudes below 40º (e.g., tropical regions). Many aspects differ between these studies
(e.g., sampling and isolation method) which makes direct comparison difficult; however, when
viewed as a group we are able to make some generalizations about the abundance and distribution
of Metarhizium spp. in different environments, several of which I would like to briefly outline:
First, Metarhizium spp. tend to be less abundant in colder regions than in temperate regions (Inglis
et al., 2008; Klingen et al., 2002; Vanninen, 1995), this observation is also supported by laboratory
work which has demonstrated that most species of Metarhizium , with the exception of M. frigidum,
do not grow at cold temperatures (Fernandes et al., 2010a; Fernandes et al., 2008). Second,
Metarhizium is more abundant than other entomopathogenic fungi in cultivated fields and open
meadows (Bidochka et al., 1998; Quesada-Moraga et al., 2007; Sun et al., 2008; Vanninen, 1995).
Third, Metarhizium is primarily found in the soil environment and not on above ground substrates
(Meyling et al., 2011; Vega et al., 2012). Lastly, Metarhizium spp. distribution tends to associate
with habitats and not with host insects (Bidochka et al., 2001; Fisher et al., 2011; Wyrebek et al.,
2011). Traditionally, insect association was thought to be the key factor in determining population
structure (Bridge et al., 1997; St. Leger et al., 1992), this shift away from the traditional paradigm
has led to many questions about what role these fungi truly play in the environment (Bidochka et
al., 2001; Vega, 2008).
Another interesting observation we can glean from viewing these studies together is that
Metarhizium spp. composition and dominance appears to be location specific. For example, a study
in the mid-east part of Canada found M. robertsii to be the most common species of Metarhizium
(Wyrebek et al., 2011), while a study in the western part of Canada found M. anisopliae s.l. to be
most common (Inglis et al., 2008). Even in Denmark survey studies have yielded inconsistent
species compositions. In 1995 Steenberg reported that M. anisopliae s.l. dominated cultivated soils
(Vega et al., 2012), also Steinwender et al. (2014) primarily found M. brunneum (a species within
the M. anisopliae complex) to be most often isolated from agricultural soil in Denmark. However,
Meyling and Eilenberg (2006) found that M. anisopliae s.l. was almost absent in a single organic
agroecosystem sampled. Also, as reported in Manuscript 3, we found that in three separate
agricultural areas, M. flavoviride was the most frequently isolated species. While further sampling
is needed to confirm these observations, it is clear that Metarhizium spp. occurrence is neither
random nor ubiquitous.
20
Table 2: Metarhizium abundance and distribution studies.
Country
(latitude) Reference
Isolation
method
Samples
taken
Habitat
types
Metarhizium
isolates
obtained General Metarhizium results
Finland
(62º N)
(Vanninen,
1995)
Insect soil
baiting
590 soil
samples
from 347
sites
Forests,
agricultural
fields
92 isolates Found in lower latitudes, not affected by
cultivation
Canada
(45 ºN)
(Bidochka et
al., 2001,
Bidochka et al.,
1998)
Insect soil
baiting
266 soil
samples
from 133
sites
Natural
(forests) and
agricultural
357 isolates Most abundant entomopathogen isolated,
most frequently recovered from soil baiting at
25ºC, more often in Agricultural soil.
Genotype association with habitat, no
association with insect host.
Norway
(66ºN)
(Klingen et al.,
2002)
Insect soil
baiting
200 samples Conventional
and organic
farms
9 isolates Not commonly found. No difference between
fields and field margins.
Denmark
(55 ºN)
(Meyling and
Eilenberg,
2006)
Insect Soil
baiting
544 soil
samples over
two years
experimental
research farm
and hedgerow
134 isolates Surprisingly low occurrence of M. anisopliae
s.l.
Spain
(40ºN)
(Quesada-
Moraga et al.,
2007)
Insect soil
baiting
244 samples Natural and
cultivated areas
71 isolates Most common in cultivated areas. Preferred
soil with low clay content.
Canada
(45 ºN)
(Inglis et al.,
2008)
Insect soil
baiting and
selective media
250 soil
samples
Urban,
agricultural and
forest
250 isolates Metarhizium very widespread and diverse
however one genotype dominated.
China
(40ºN)
(Sun et al.,
2008)
Insect soil
Baiting
>2300 soil
samples
cultivated fields
and orchards
60% of soil
samples
More frequent in cultivated fields than
orchards.
South
Africa
(33ºS)
(Goble et al.,
2010)
Insect soil
baiting
288 soil
samples
Conventional
and organic
citrus farms
16 isolates No difference between organic and
conventional.
USA
(44 ºN)
(Fisher et al.,
2011)
Insect baiting
with roots
339 root
samples
Strawberries,
blueberry,
grapes, and
Christmas trees
(roots)
94 isolates Species/ plant-root association; M. brunneum
= strawberries and blueberries, M.
guizhouense = Christmas trees, and M.
robertsii = Christmas trees
Canada
(45 ºN)
(Wyrebek et al.,
2011)
Washed root
homogenate on
selective media
200 root
samples
Natural
meadows, and
forests (roots)
102 isolates Species/ plant-root association; M. brunneum
= shrubs and trees, M. guizhouense = tree
roots, and M. robertsii = grasses and
wildflowers
Denmark
(55 ºN)
(Steinwender et
al., 2014)
Insect soil
baiting
53 soil
samples
Agricultural
field and
boarding
hedgerow
123+ isolates Five genotypes of M. brunneum , 6
genotypes of M. robertsii. One M. brunneum
genotype most dominant.
Denmark
(55 ºN)
Keyser. et al.
(2015) –
Manuscript 3
Insect soil
baiting and
selective media
450 soil and
root samples
Winter wheat,
Oilseed rape
and natural
meadow
132 isolates 118 of the isolates were M. flavoviride, 13 M.
brunneum and 1 M. majus. AFLP analysis
revealed high level of diversity with the M.
flavoviride species
21
2.2.2. Abiotic factors that affect survival and growth
Three of the most important abiotic factors that affect entomopathogenic fungal
performance are: temperature, humidity, and UV-radiation. Temperature has been shown to affect
Metarhizium spp. germination, hyphal growth and infection rates (Keyser, 2010; Keyser et al.,
2014a). Growth at high and low temperatures has even been used as phenotypic traits to distinguish
certain species of Metarhizium (Fernandes et al., 2010a). Fluctuating ambient temperatures have
also been indicted as one of the primary limiting factors in field success (Foster et al., 2010; Foster
et al., 2011). Likewise, relative humidity is an important factor in determining growth, infection,
sporulation and conidial longevity (Arthurs and Thomas, 2001; Daoust and Roberts, 1983; Milner et
al., 1997; Vega et al., 2012). UV radiation, especially UV-B radiation can be highly detrimental to
conidia survival (Braga et al., 2001; Rangel et al., 2005) and even sub-lethal UV-B radiation
exposure was observed to delay conidial germination (C.A. Keyser, unpublished data). These
factors are also highly relevant in understanding the natural distribution and abundance in the field.
Some species of Metarhizium have been shown to be less cold tolerant then Beauveria spp.
(Fernandes et al., 2008), which may explain why Vanninen (1995) found Metarhizium primarily in
the southern Finland areas while Beauveria was isolated all over Finland. In one area of southern
Alberta, Canada, Inglis et al. (2008) did not find any Metarhizium isolates, they suggested that a
possible explanation for the lack of isolates is that the area surveyed was semi-arid, had very cold
winters and short summers. Bidochka et al. (2001) also observed that isolates found in forested
areas were more likely to grow at low temperatures while those found in open fields showed a
propensity for growth at higher temperatures and UV-B tolerance. Abiotic factors have strong
influence on Metarhizium population structure and biological success.
One of the challenges that has slowed BCA implementation is that they are sometimes
viewed (especially by the end user) to be one-to-one substitutions for chemical pesticides (Cook,
1993). This leads the expectation that they will have a similar shelf life, can be applied in similar
conditions, and will have a similar mode of action and time to kill. Distinguishing the differences
between applying a living organism and a chemical is vital to successfully integrate BCAs as a
viable treatment option. One of the limitations is BCA susceptibility to abiotic environmental
factors (Jaronski, 2010; Starnes et al., 1993). Future research that uncovers the mechanisms and
limitation regarding responses to abiotic factors will greatly aid in improving BCA effectiveness.
22
2.2.3 Environmental dissemination pathways
Fungi are non-motile organisms, in nature the infection propagules (e.g., conidia) of
Metarhizium are dispersed passively. Generally dispersal is thought to occur by abiotic factors such
as wind and rain (Hajek, 1997; Inglis et al., 2001; Meyling and Eilenberg, 2007). Additionally, it is
possible that insects as well as other animals may act as vectors for conidia (Meyling et al., 2006).
In Manuscript 1 we show that plants also act as a vector in aiding conidia dispersal through the soil
environment (Keyser et al., 2014b), and we speculate that this may explain why entomopathogenic
fungi have evolved to associate with plants (see also section 3). Historically, biological control
programs utilizing Metarhizium as a bio-pesticide have tried to adapt chemical-pesticide application
methods for conidial dispersal (Bateman, 1997) (Figure 3). Often formulating conidia for
application in liquid substrate or as a powder, this is then applied topically to vegetation (Booth et
al., 2000; Caudwell and Gatehouse, 1996; Griffiths and Bateman, 1997).
The effectiveness of biological control programs using Metarhizium have been inconsistent,
one factor that may be contributing to the unpredictability of Metarhizium as a BCA is the
application method or delivery system. Several studies have shown that application method does
greatly influence infection rates and environmental persistence (Farenhorst et al., 2008; Fargues et
al., 1997; Jenkins and Thomas, 1996; Kanga et al., 2003); however nearly all of these studies are
focused solely on the BCA implementation and thus neglect further investigations to understand the
underlying ecological principles contributing to increased infectivity. Understandably, designing
Figure 3. Methods of Metarhizium application. (A) In China mortar shells filled with powdered conidia were launched above a forested area using a grenade launcher (photo by Richard Soper), arrow indicates conidial cloud. (B) Conidia formulated in oil is applied to grasshopper infected rangeland in Utah, USA, using a rear-mounted sprayer (photo by C. A. Keyser).
23
BCAs to fit seamlessly into insecticide application methods greatly enhances their usability and
facilitates an easy transition away from chemical pesticides. Unfortunately, without an
understanding of the natural dispersal mechanisms which contribute to efficacy, consistent
biological control results will be more a matter of luck than design. Only by investigating the
ecological principles can we hope to improve reliability. For example, in a study to evaluate the M.
brunneum biocontrol product Met52 for control of Black vine weevil, Otiorhychus sulcatus (Col.
Curculionidae) in field grown strawberries, Ansari and Butt (2013) tested several application
methods using the granular formulation of the commercial product. The methods of application
included: 1. Premixed in soil; 2. Drench application to the base of each plant; and 3. Plant roots
being dipped in an aqueous suspension of the conidial product and then planted. They found that
Black vine weevil control was more efficient when the drench application method was used.
Further studies revealed that plant roots were colonized by significantly more conidia than when the
drench method was used (Ansari and Butt, 2013). This additional information allowed them to
conclude that the conidia concentration in the rhizosphere was a key component to improving
infectivity. It was recently shown, however that M. brunneum population dynamics in the
rhizosphere may depend on adaptations to the local environmental conditions; a Norwegian M.
brunneum isolate proliferated more in strawberry rhizopheres at ambient temperatures in Norway
than an isolate similar to Met52 which originated from Austria (Klingen et al., 2015). Clearly,
understanding how infectious propagules are dispersed naturally can improve BCA performance in
the field.
3. Trophic interaction
One of the greatest challenges to fully understanding the ecology of the world we live in is
accounting for all the trophic interactions that influence an organism; however for BCAs it is
crucial that we account for these interactions as they will greatly affect efficiency. If we truly hope
to exploit biological control to suppress pests, we must view insect pathology not as one organism
acting on another, but rather as a node in a complex web of intertwined organisms and response
variables which have co-evolved and adapted to each other. This can only be achieved by studying
the organisms in combination and not individually and valuing both direct and indirect interactions.
The following sections will highlight several key interactions that occur between
Metarhizium and other important organisms (Figure 4). Some of these interactions have been well
studied (e.g., Metarhizium ↔ Insects), while for others very little is known (e.g., Metarhizium ↔
Other microorganisms ↔ Plants). The overall message that I hope to convey is the importance of
24
not only understanding the various responses associated with individual bi-trophic interactions, but
also a broad perspective of how they affect each other.
Figure 4: Illustration depicting several trophic interactions that may occur between Metarhizium
spp. and other organisms. Blue arrows represent direct interactions and orange arrows represent
indirect interactions. Diagram by C. A. Keyser
3.1 Metarhizium ↔ Insects
Among the millions of fungal species in the world, Metarhizium spp. have garnered
significant scientific and economic interest primarily because of how they interact with arthropods.
A large portion of the research involving Metarhizium centers on its use as a BCA and consequently
25
deals with its relationship to various insects. As a generalist, many Metarhizium spp. are able to
infect a wide range of hosts (Veen, 1968; Zimmermann, 1993), however the virulence can vary
considerably between different host species (Butt et al., 1992), making it necessary to test virulence
towards each insect species of interest. Furthermore, virulence varies between isolates even within
the same fungal species (Keyser, 2010), which further complicates the selection of appropriate
isolates for BCA use. The variation in virulence should not necessarily be looked at as a negative
aspect for a potential BCA; it is important to remember that a very small percentage of all insect
species are important pests – many herbivores do not cause any economic damage and some
predators, parasitoids and pollinators are important beneficial insects. The variation in host
virulence allows selection for a BCA that is highly virulent to a particular pest insect while being
less virulent to non-target insects. For example, Falagiarda (2014) observed that a commercial
isolate of M. brunneum, the same isolate used in Manuscript 1 and 2, to be highly virulent to the
grain-pest insect T. molitor but having very low virulence to the beneficial coleopteran, Atheta
coriaria (Figure 5). Her results suggest that this isolate of M. brunneum could therefore be
considered a “low risk” substance under the proposed EU legislation. Further testing might
investigate whether there is an additive or synergistic effect when M. brunneum and A. coriaria are
used in combination as BCAs.
Many factors from both the host and the pathogen contribute to virulence; it is a give and
take relationship with each attempting to maximize their own fitness. Each step in the infection
process (see Figure 2) is controlled by specific cues and responses which determine the success of
the infection. For example, ambient pH levels on and around the insect cuticle regulate the
secretion of proteolytic and chitinolytic enzymes which aid in the penetration process (St. Leger et
al., 1998). In response to the infections, insects have evolved different immune responses, both
physiological and behavioral, to mitigate the pathogenic effects. For example, after exposure to
Metarhizium there are changes in insect biochemistry, including melanization of the cuticle and
antimicrobial defenses of the haemolymph (Dubovskiy et al., 2013; Gillespie et al., 2000). Also,
behavioral adaptations have been noted, including: increased grooming among infected ants and
termites (Hughes et al., 2002; Qiu et al., 2014; Yanagawa et al., 2008), or basking in the sun in
order to elicit a “behavioral fever” which restricts or kills the infecting pathogen (Blanford and
Thomas, 2001; Kemp, 1986; Ouedraogo et al., 2004). These immune responses can severely limit
the effects of a pathogen; however some species of Metarhizium have developed traits to more
efficiently overcome insect immunity. For example, to increase virulence many of the generalist
26
species of Metarhizium produce cyclic peptides known as destruxins (Roberts and St. Leger, 2004);
these insecticidal toxins cause muscle paralysis and suppress immunoresponses in the host (Pedras
et al., 2002; Roberts, 1981).
These examples represent only a small fraction of the many interactions that take place
between insects and Metarhizium; however, they begin to illustrate the complex dance that occurs
between host and pathogen. The level of complexity can be even greater when multiple trophic
levels of insects are considered. For example, Rännbäck et al. (2015) observed a reduction in
parasitoid egg laying when hosts were infected with Metarhizium. While the complexity of these
interactions can seem overwhelming, it is highly relevant that we understand what is occurring if we
hope to successfully implement BCA to control pest insects.
3.2 Metarhizium ↔ Plants
Most land plants form symbiotic relationships with soil fungi (van der Heijden et al., 1998).
It is therefore not surprising that several species of Metarhizium have been observed to interact with
some plants. A fungal endophyte is defined as an asymptomatic plant-colonizing fungus that lives a
portion of its life cycle inside the plant (Behie and Bidochka, 2014a). Metarhizium spp. have a dual
life cycle, persisting in the environment both as an insect pathogen and as a facultative saprophyte
(Wang et al., 2005). While soil has long been considered a reservoir for naturally occurring
Metarhizium, it has not been clear whether the recovered isolates were from dormant conidia in the
soil or hyphae actively growing on plant material (St Leger, 2008). Metarhizium has been viewed
for many years as only an insect pathogen – the realization that it also actively interacts with plants
a b
Figure 5. Bioassay survival curves after exposure to Metarhizium brunneum or Beauveria bassiana of
(a) Tenebrio molitor larvae and (b) Atheta coriaria after exposure to M. brunneum (Falagiarda, 2014).
27
is both novel and exciting for the field of Metarhizium research. For this reason and because it is of
special interest to the research contained in this thesis, I will give a more comprehensive outline of
the current status on Metarhizium ↔ Plants interactions.
As mentioned in section 2.2.1, specific species of Metarhizium have been shown to associate
closely with different plants. In a Canadian-field survey Wyrebek et al. (2011) observed that M.
robertsii was the only species associating with grass roots, while M. guizhouense tended to
associate with roots of trees and M. brunneum was found in the roots of shrubs and trees. In a
similar study Fisher et al. (2011) found that in Oregon, M. brunneum associated strongly with roots
of Strawberry and Blueberry plants while M. robertsii and M. guizhouense were isolated
predominantly from Christmas tree roots. The plant specificity observed in these two studies could
indicate a history of co-evolution between Metarhizium and certain plants.
The rhizosphere is a region of soil where plant-root exudate influences soil microorganisms.
M. anisopliae s.s was first discovered to be a rhizosphere competent isolate by Hu and St Leger
(2002) in a field study designed to evaluate the fate of the BCA after application. In a cabbage field
soil samples were collected 4-5 cm from the plant as well as directly next to the taproot. The
researchers observed that even after a year the population of M. anisopliae s.s. remained high in the
rhizosphere area while it declined over time in the bulk soil (Hu and St Leger, 2002). M. brunneum
was also observed to be rhizosphere competent in soilless potting media (Bruck, 2005) and several
Metarhizium spp. isolates have been shown to germinate and grow in root exudates (Pava-Ripoll et
al., 2011; Wang et al., 2005). Additionally, specialized genes which become active when
Metarhizium interacts with plants or plant compounds have been identified; like, the Mad2 gene
which is involved in adhesion to plants during colonization (Barelli et al., 2011; Wang and St
Leger, 2007), or the Mrt and Mlrnv genes which transport oligosaccharides found in root exudate
(Fang and St Leger, 2010; Liao et al., 2013). These studies clearly show that Metarhizium is more
than just an entomopathogen but that it has evolved to propagate while interacting with plants.
In an effort to determine if Metarhizium had a localized plant-tissue preference when
associating with plants in the field Behie et al. (2015) performed a field survey of grasses and forbs
in Canada. They found that endophytic Metarhizium spp. (95% of which were M. robertsii)
associations were exclusively with plant roots and not with hypocotyl or the stem and leafs of a
plant. In vitro laboratory studies with Haricot beans also showed endophytic root preference of
Metarhizium spp. (Behie et al., 2015). However, Batta (2013) was able to re-isolate M. anisopliae
s.s from untreated leaves, petioles and stems of the oilseed rape plants when other leaves were
28
sprayed with a high dose of M. anisopliae. Furthermore, Golo et al. (2014) observed that cowpea
and cucumber plants resulting from M. robertsii or M. acridum inoculated seeds had endophytic
association in both the roots and leaves of the plants after 12 days. They further observed the
production of destruxins by M. robertsii in the cowpea plants.
Akello and Sikora (2012) showed that M. anisopliae s.s. could live for at least a month
inside V. faba roots as an endophyte after seeds were soaked for 4 hours in a conidial suspension.
Interestingly, in a similar study Akutse et al. (2013) did not observe M. anisopliae s.s. colonizing
any part of V. faba plant when seeds were inoculated with a conidial suspension even though the
same fungal isolate and plant were used as well as similar methods as Akello and Sikora (2012);
although in addition to treating the seeds with conidia (as was done in Manuscript 1), Akello and
Sikora (2012) also drenched soil with a conidial suspension, the additional load of conidia in the
soil might explain why an endophytic interaction was observed in one and not the other.
Further implications regarding the importance of Metarhizium ↔ Plants interactions were
suggested when, in a proof of concept study, Behie et al. (2012) showed that nitrogen from a M.
robertsii-infected insect can be transferred to a plant via an endophytic hyphal connection. In a
follow-up, in-depth study Behie and Bidochka (2014b) tested the insect-derived nitrogen-
transferring abilities of five species of Metarhizium [i.e., M. acridum, M. brunneum, M. pemphigi
(=flavoviride var. pemphigi), M. guizhouense, and M. robertsii] to four types of plants (haricot
bean, soybean, switchgrass and wheat). They showed that all five Metarhizium species had the
capacity to transfer nitrogen to plants, although in varying degrees. In addition, they showed that
nitrogen was also transferred in the field, despite other competing microorganisms (Behie and
Bidochka, 2014b).
Metarhizium-plant associations have also been observed to promote plant growth. Sasan
and Bidochka (2012) observed that after inoculation with M. robertsii, switchgrass and haricot bean
plants both had increased root hair growth. Also, increased plant growth has been observed in
several agricultural crops, including soy bean (Khan et al., 2012), tomato (Elena et al., 2011), and
corn (Liao et al., 2014). In soy bean, Khan et al. (2012) observed endophytic interaction with M.
anisopliae s.l. increased biomass, chlorophyll contents, transpiration rate, photosynthetic rates and
leaf area compared to untreated control plants. While wild type M. robertsii, M. brunneum and M.
anisopliae s.s. increased many aspects of corn growth, Liao et al. (2014) observed that when
Metarhizium genes that are associated with either adhesion to the plant or the utilization of plant
exudates were knocked out, no plant growth promotion was observed.
29
The ecological significances of delving in to the complex systems of the Metarhizium ↔
Plants interactions are clear. Furthermore, these fundamental research studies also have important
implications for biological control. Nearly all the studies so far have described either beneficial or
neutral effects on the plant resulting from Metarhizium associations. Based on the results of these
studies, Metarhizium based BCA may do more than just protect crops from insect pests, they may
also aid in nutrient acquisitions and plant-growth promotion. However, more research is necessary
to illuminate the mechanisms involved in these processes and whether the benefits observed in the
laboratory are also seen in the field.
Thus far, the majority of the published studies involving Metarhizium ↔ Plants interaction
have focused on responses exhibited by the plant. This is most likely because traditionally
underlying justification for Metarhizium research has been in the interest of plant protection,
however, research into beneficial or deleterious effects to the fungal organism should also be of
interest. In Manuscript 1, after demonstrating that species of Metarhizium will disperse along a
growing root though soil, I suggest that a possible benefit that Metarhizium derives from associating
with plants is mobility and proximity to potential hosts. It is likely that the fungus is also affected
in other ways while interacting with plants so it is important that questions like, “Why would a
Metarhizium organism give up a limited resource such as nitrogen and what does it receive in
return”, continue to be investigated. Metarhizium ↔ Plants interactions are an important part of the
future of biological control research.
3.3 Metarhizium ↔ Other microorganisms
Very few studies have been conducted to investigate the interaction between Metarhizium
and other microorganisms. This is an important aspect of Metarhizium ecology that should be
addressed more thoroughly. Metarhizium spp. are abundantly found in the soil environment
(Tkaczuk et al., 2014). It is likely that an actively growing saprophyte will have developed
antimicrobial strategies to survive and compete in an environment teaming with natural
microorganisms. I observed evidence of this while performing isolation on nutrient agar.
Inadvertently, a petri plate which had been inoculated with a new isolate of M. flavoviride also
became contaminated with a fast growing unknown fungus, however a very clear inhibition zone
was present between the M. flavoviride and the contaminate (Figure 6a). Additionally, while
developing the methodology for Manuscript 2, media plates with M. brunneum, M. robertsii and M.
flavoviride were also inoculated with plugs of Fusarium culmorum. A small zone of inhibition was
observed on the plates with M. brunneum and M. robertsii and a much larger zone was present on
30
Figure 6: Inhibition zones observed between Metarhizium spp. isolates and other fungi on PDAY media. (A) M. flavoviride isolate from bait insect on petri plate with un-known fungal contaminant. (B) M. brunneum, M. robertsii, and M. flavoviride on petri plate with Fusarium culmorum.
those with M. flavoviride (Figure 6b). Sasan and Bidochka (2013) also observed a zone of
inhibition when M. robertsii and Fusarium solani were cultured on the same petri plate and they
noted a significant reduction of the colony size of the F. solani. Furthermore, Sasan and Bidochka
(2013) showed that liquid media, which had had M. robertsii growing in it but was then passed
through a filter to remove all fungal material suppressed F. solani germination. They suggested that
this indicates that M. robertsii secretes an anti-fungal compound that inhibits F. solani growth.
Krauss et al. (2004) tested the interaction between several entomopathogenic fungi,
including two strains of M. anisopliae s.l., and mycoparasitic fungi by completely colonizing a petri
plate with the entomopathogen and then placing an agar plug of the mycoparasite on top of the
entomopathogen colony. They claimed that because the mycoparasite was not in contact with the
media any growth indicated it was receiving nutrients from the fungus and not the media. They
found that of the isolates they tested M. anisopliae s.l. was the most susceptible to mycroparasitism
and allowed growth of all the mycoparasites tested including Clonostachys byssicola, C. rosea and
Lecanicillium lecanii (Krauss et al., 2004). These two studies demonstrate that Metarhizium spp.
are both affected by and effectors of other microorganisms. Further studies with regard to the
mechanisms involved in these interactions would greatly expand our understanding of the ecology
of Metarhizium spp. in the field and identify potential benefits and challenges to their use as BCAs.
31
3.4 Multi-trophic interactions with Metarhizium
Each additional trophic level included in a study greatly increases the size and complexity of
the experiment necessary to evaluate all the variable permutations. It is therefore not surprising that
most studies focus on bi-trophic interactions. Nevertheless, multi-trophic interactions which
include three or more levels are necessary to both better grasp what occurs in nature and provide
greater predictive power to BCA employment. Generally bi-trophic interactions are concerned with
direct effects while multi-trophic interactions must account for both direct and indirect effects. In
the following section I will review several Metarhizium studies which evaluate multi-trophic
interactions. The trophic levels that I focus on are those of different types of organisms (i.e., other
microorganisms, insect and plants); however multi-trophic interactions that involve multiple species
of the same type of organism (e.g., insect ↔ insect ↔ microorganism) – as was seen above in the
study by Rännbäck et al. (2015) in which interaction between a parasitoid insect as pest insect and
M. brunneum were evaluated – should not be neglected.
3.4.1 Metarhizium ↔ Other microorganisms ↔ Insects
There are a few examples of tri-trophic interaction involving Metarhizium, other microbes
and insects; generally they are geared towards evaluating how the biological control capacity of
Metarhizium is affected when other microorganisms are present. Hughes and Boomsma (2004)
found that the normally avirulent, opportunistic fungal pathogen Aspergillus flavus would out-
compete a highly virulent isolate of M. anisopliae s.l. when applied as a mixture on a leaf-cutting
ant host. They explained that alone A. flavus is generally unable to overcome the host immune
defenses, however, when coupled with a second pathogen like Metarhizium, which is more adept at
suppressing the immune responses, the avirulent fungus is then able to grow much faster and better
utilize the pilfered resources. Geetha et al. (2012) demonstrated that co-application of multiple
fungi on the same insect host negatively influence the virulence and sporulation of M. anisopliae s.l.
Also, Krauss et al. (2004) found that when applied in combination with mycoparasitic fungi on
three different species of insects, the virulence of M. anisopliae s.l. was not significantly affected,
despite the authors having found that M. anisopliae s.l. was highly susceptible to mycroparasitism.
In Manuscript 2, an insect bioassay was conducted in which Tenebrio molitor larvae were
inoculated with one of three species of Metarhizium (M. brunneum, M. flavoviride s.s., or M.
robertsii) combined with either the mycoparasite Clonostachys rosea or the plant pathogen
Fusarium culmorum or both. We observed that, when compared to the individual treatments, for
some of the combined treatments there was a slight reduction in virulence; however, in general,
32
virulence remained similar to the individual Metarhizium treatments. Based on this study and the
others mentioned it is obvious that interaction which affect the BCA performance of Metarhizium
occur when other microorganisms are present. Since microbes are always present in the field these
interactions are highly relevant – especially those with other BCA like C. rosea which are also often
applied for crop protection.
3.4.2 Metarhizium ↔ Other microorganisms ↔ Plants
In light of the recent emphasis placed on Metarhizium ↔ plant interactions, the tri-trophic
interaction between Metarhizium, other microorganisms and plants are highly relevant. There have
been very few studies which have looked at these interactions. Sasan and Bidochka (2013) found
Haricot bean seeds had higher germination when in the presence of M. robertsii and F. solani than
when only F. solani was present. The resulting plants also showed significantly less F. solani
infection symptoms when M. robertsii was also present. In Manuscript 2 we also evaluate the
interactions between Metarhizium (M. brunneum or M. flavoviride), C. rosea, F. culmorum and
Winter wheat. We observed that the presence of either of the Metarhizium species did not reduce
the F. culmorum infection or hinder the biocontrol efficacy of C. rosea. The two beneficial BCAs
may therefore potentially be used in concert against both insect pests and plant pathogens without
obstructing each other’s effects. But no additive nor synergistic effects should be expected
(Manuscript 2). Several important differences exist between Manuscript 2 and the study by Sasan
and Bidochka (2013) which might account for the different observations. For example, the species
of Metarhizium and Fusarium that were used are different, as was the plant species and inoculation
method; also Sasan and Bidochka (2013) allowed an establishment period for M. robertsii and F.
solani in the soil before introducing the bean seeds, where as in Manuscript 2, un-germinated seeds
were exposed to F. culmorum first and then Metarhizium spp. before germination.
3.4.3 Metarhizium ↔ Plants ↔ Insects
The indirect effects to plants are nearly always implied in Metarhizium ↔ insect studies
which have a biological control aspect to them. Nevertheless these indirect effects (i.e. increased
plant productivity caused by reduced effects of pest insects after BCA application) are often not
measured. One example is a study by Kabaluk and Ericsson (2007) in which they found that corn
seeds treated with the M. brunneum BCA F52 (called M. anisopliae by the authors) resulted in an
increased yield in comparison to untreated control plants when planted in fields with wireworm. On
the other hand, indirect effects may also be observed to occur to the insect when the plant interacts
with Metarhizium. For example, Akello and Sikora (2012) showed that aphids feeding on V. faba
33
plants which had been treated as seeds with different fungi including Metarhizium spp. had reduced
survival, offspring fitness, development and fecundity compared to untreated control. They
demonstrated that Metarhizium spp. isolates along with other endophytic isolates indirectly
protected the plant from aphid damage. However, the mechanisms behind this remain unknown.
3.4.4 Metarhizium ↔ Other microorganisms ↔ Plants ↔ Insects
The last type of interaction that I would like to mention is that which involves four or more
trophic levels. Very few studies have attempted to incorporate so many different trophic levels; in
fact I was unable to identify any other studies, involving Metarhizium, which evaluated response
variables for four trophic levels. One example, which uses another entomopathogenic fungus (B.
bassiana) tested whether insect pollinators could be utilized as delivery vehicles to vector two
BCAs to plants in order to control both an insect pest and a plant pathogen (Kapongo et al., 2008).
They found in laboratory greenhouse trials that the bees successfully vectored the BCAs to the
flowering plants and they observed a reduction in both plant pathogen and insect pest occurrence.
Manuscript 2 also describes a system with up to five trophic levels are evaluated. F.
culmorum infected seeds were treated with C. rosea, a mycoparasitic fungus which can be used as a
BCA against plant disease, and two Metarhizium spp. isolates. After the plants had grown for 14
days the roots were feed to T. molitor larvae which were then monitored for mortality and fungal
disease. There were two main response variables assessed in this study, plant disease incidence and
insect mortality. Combination effects could be assessed by comparing the data of the combination
treatments with those of the non-combined treatments.
Prior to this experiment we had several hypotheses on what combination effects we might
expect. Metarhizium has been shown to have antifungal properties (Sasan and Bidochka, 2013) and
therefore might aid in Fusarium disease suppression. As a potential mycoparasite of Metarhizium
spp. (Krauss et al., 2004), C. rosea may severely reduce the ability of Metarhzium to disperse along
the root and subsequently infect the larvae. On the other hand, isolates of Fusarium spp. and C.
rosea have been observed to be pathogenic to insects (Teetor-Barsch and Roberts, 1983; Vega et al.,
2008), and may therefore have an additive effect on insect virulence when in combination with
Metarhizium spp. As reported in Manuscript 2, no effect on plant-disease reduction by C. rosea
was observed when Metarhizium was added, however when C. rosea was present, alone or
combined with Metarhizium spp. there was little to no disease symptoms in the plants; the high
efficiency of the C. rosea treatment may however have masked any positive effects of Metarhizium.
In most of the treatments there was a significant reduction in virulence to the insect when the seeds
34
had been treated with Metarhizium spp. combined with another fungus. This indicates that there is
an indirect effect on insect virulence when other fungi are present. Future studies should evaluate if
this effect is due to direct interaction between the combined fungi or due to an indirect effect like
resource competition. It is clear however, that multi-trophic interactions are important and may
yield unexpected results.
4. Methodology
In fulfilling the research requirements of this thesis it was necessary that I develop and test
various experimental methodologies and expand my analytical skills. The following section will
briefly summarize and describe a few important methodological techniques I worked with.
4.1 Selective media
Selective media is often used to assist in the isolation of entomopathogenic fungi. The basic
principle of selective media is to provide a substrate that allows the growth of a desired organism
while discouraging the growth of others. This can be accomplished in several ways, for example,
many bacteria are inhibited by low pH levels while fungi are not. Also the nutrient composition of
many growth media favor particular organisms, e.g., Potato dextrose media and Sabouraud dextrose
media are better suited for fungal growth than bacterial. While usually not included as a selective
medium, insects used for the soil baiting method (Zimmermann, 1986) are essentially a “ready-
made” selective medium that screens out any non-pathogenic organisms and selects for those that
can infect the host.
Media are often amended with more specific growth inhibiting components to further select
for desired organisms. Antibiotics, like streptomycin or chloramphenicol, can be added to help to
reduce contaminating bacteria. Contaminating fungi are more problematic. For many species of
Beauveria and Metarhizium some fungicides, like dodine or cyclohexamide, in low concentration
help to eliminate the fast growing contaminants like Rhizopus or Trichoderma while allowing
Metarhizium and Beauveria growth (Fernandes et al., 2010b; Rangel et al., 2010) (Figure 7). Many
different media have been developed for the isolating of Metarhizium spp.; Table 3 lists some of the
major component combinations that have been found effective as well as the studies in which they
were presented.
35
Figure 7: Selective media test with several types of media (columns) to evaluate effectivness at
supressing naturally occuring microbes while allowing the growth of entomopathogenic fungi.
Both natural and Metarhizium “spiked soil” was used (rows). Soil was diluted in ddH2O and then
200µl was pipetted onto each plate. Plate incubated for 21 days at ~21ºC.
36
Table 3: Selective media ingredients that have been observed to be effective for the isolation of
Metarhizium spp isolates from soil. All concentratoins represent grams/liter unless otherwise
specified.
Media Ingredients Ve
en
& F
err
on
, (1
966
)
Be
ilharz
et
al.,
(198
2)
Ch
ase
et
al.,
(19
86
)
Liu
et
al.,
(199
3)
Sh
imazu
& S
ato
, (1
996
)
Str
asse
r e
t a
l., (1
997
)
Hu
gh
es e
t a
l.,
(20
04
)
Sh
in e
t a
l.,
(201
0)
Re
ng
al e
t al.,
(20
10
)
Fe
rna
nd
es e
t al.,
(20
10b
)
Wyre
be
k e
t a
l.,
(20
11
)
Ro
ch
a &
Luz,
(201
2)
Ste
inw
end
er,
(2
013
)
Ke
yse
r e
t a
l.,
(20
14
b)
Se
lec
tive
In
gre
die
nts
Dodine 0.065 0.46* 0.01* 1ml* 0.1 0.05 0.02 0.325 0.300 0.29 0.2
Cycloheximide 0.25 0.25 0.05 0.25 0.5 0.06 0.25
Chloramphenicol 0.5 0.5 0.05 0.5 0.2 0.014 0.5
Thiabendazole 0.001
Chlortetracycline 0.005 0.005
Copper chloride (CuCl2) 0.02
Gentamicin
Streptomycin 0.6 0.1 1
Penicillin 0.4
Tetracycline 0.05
Crystal violet 0.01 0.01 0.01 0.01
Nu
trie
nt
Ing
red
ien
ts
PDA X X X X
SDA 30% X X X
Yeast extract 1 1 X
Glucose 10 10 20
Peptone 10 10 10
Oxgall 15 15
Oatmeal infusion 20 20 20
Agar 35 20 20 35 18 20
pH 10+ 6.9 6.9
37
4.2 Bioassay statistics
A bioassay is a scientific study with the aim to determine the biological activity or potency
of a substance by testing its effect on the growth of an organism. In insect pathology an infection
bioassay is a study which evaluates the infectivity of a particular pathogen on a host insect. The
ability to cause infection in insects is one of the most basic and interesting traits of
entomopathogenic fungi like Metarhizium spp. It is for this reason that many studies of these fungi,
among other things include infection bioassays. Infection bioassays are often designed to evaluate
pathogenicity, the ability to cause infection, and virulence, the killing power of a pathogen.
The most common type of studies that include infection bioassays are those aimed at
determining the biological control potential of a pathogen for a particular host. However, infection
bioassays are regularly included in other types of studies as a phenotypic trait that can be used to
compare different genotypes to each other or measure changes within the same isolate after a
mutation or stress. For example Jin et al. (2012) used infection bioassays to show the effects of the
Hog1-type mitogen-activated protein kinase gene in M. acridum, or Lopes et al. (2013) who while
performing a diversity study of Beauveria spp. and Metarhizium spp. in banana fields included a
bioassay and interpreted low virulence to explain the low occurrence of epizootics. For any insect
pathologist an understanding of how to appropriately design and execute an infection bioassay is a
vital skill.
4.2.1 Experimental design
There are several factors that influence the outcome of an infection bioassay; however, the
two most important factors are time and dose. Therefore, experiments are usually designed around
these factors either as dose-mortality or time-mortality experiments. In a dose-mortality experiment
the pathogen dose or number of conidia administered to each host is varied while the time at which
the response is evaluated is kept constant. Often in a dose-mortality experiment the response is
reported as a value of LD50 or LD90 (dose at which 50% or 90% of individuals exhibit the desired
response, i.e., mortality) for a particular treatment. The most important factors are sample size and
dose range. It has been recommended that sample size of 120 to 240 insects is necessary to obtain a
reliable response (Robertson et al., 1984). Ideally the dose range will include three to eight doses
that result in 25 to 75% responses at the time of observations (Robertson et al., 1984), however, the
experiment can be checked at several time periods and then the most appropriate observation time
for the analysis can be selected afterwards.
38
In a time-mortality experiment, dose is kept constant (or multiple doses are considered
separately) and the response is measured over a period of time, often results are reported as LT50 or
LT90. To avoid data being correlated in a time-mortality experiment, either different groups of
insects must be used for each time measurement so that the data are not correlated or the method of
analysis must allow for correlated data. The bioassay performed in Manuscript 1 and 2 were
designed as time-mortality experiments with the data for each dose being analyzed separately.
I conducted a survey of 30 randomly selected scientific publications selected from a Google
Scholar search with the key words “Metarhizium” + “Bioassay” and limited to papers published
between Jan 2010 and April 2014. Of these 30 papers, 15 included time-mortality bioassay designs,
7 dose-mortality experiments and 8 with both (Table 4).
4.2.2 Types of Statistical Analyses
4.2.2.1 Abbot correction: Random mortality not related to a treatment but rather
experimental conditions being tested in an infection bioassay can be adjusted for in the analysis
using the control group. The most common method employed in insect pathology is the Abbot’s
formula (Abbot, 1925). The following formula is used to estimate the percentage of insects killed
by a particular treatment: 𝑃 = (𝐶−𝑇
𝐶) ∗ 100. Where P is the estimated percentage of insect mortality
due to treatment, C is the percentage dead in the control and T is the percentage of dead in
treatment. A few considerations before implementing an Abbot adjustment include: First, the
Abbot formula assumes pathogenicity of a treatment, and therefore should not be used if the
researcher wishes to determine if a particular treatment differs from the control. Second, if a
control has greater mortality than a treatment an Abbot correction will result in negative percent
mortality and is not appropriate. Lastly, an Abbot correction cannot be used when performing a
survival analysis because the binomial data used for the analyzed is of the individual and not the
group.
4.2.2.2 Probit analysis: Infection bioassays are typically analyzed in one of two ways, the
first is using a probit analysis model. A probit analysis is most appropriate for dose-response
designs but can be used in a time-response design if different groups of insects are used for each
time measurement otherwise the data are correlated and the model is not valid; however, examples
have been shown where correlated data can be analyzed using a probit transformation of proportion
of insects killed (Goettel and Inglis, 1997).
Probit analysis is a type of regression used to analyze binomial response variables. It
transforms the sigmoid dose-response curve to a straight line that can then be analyzed by linear
39
regression analysis. Probit analysis was first published in 1934 by Chester Bliss, an entomologist
working with pesticides and their effectiveness for pest control (Bliss, 1934). Later in 1952 David
Finney, a professor of statistics, published a book called Probit Analysis (Finney, 1952). Probit
analysis continues to be one of the preferred statistical methods in understanding dose-response
relationships.
4.2.2.3 Survival analysis: The survival analysis is historically one of the oldest fields of
statistics dating as far back as the 17th
century (Aalen et al., 2009). As suggested in the name, a
survival analysis traditionally is used to analyze survival or death rates, however today it is often
used in engineering to predict failure times of machines. A survival analysis is used to analyze data
in which time duration until an event is of interest occurs. The response is often referred to as a
failure time, survival time, or event time. One of the primary advantages of using a survival model
is that it has the ability to account for censored data, most statistical models don’t. Censored data is
data in which the response is unknown in the window of observation, for example, if an experiment
ends before all the individuals are dead those individuals are considered censored. An ordinary
linear regression model cannot handle censored data. Despite its early beginnings, it was not until
the late 1950s that the field of survival analysis was significantly advanced. A publication in 1958
by Kaplan and Meier which allowed a survival curve estimation was presented and then later in
1972 Cox published a method of comparing survival curves (Aalen et al., 2009). Both of these
modeling approaches advanced the usefulness and the applicability of survival analysis to the
current state. In Manuscripts 1 and 2 bioassays were performed. The experimental design of these
bioassays in each study was based on a survival analyses. A Cox proportional hazard model was
used to compare the survival curves between the various treatments. This model was most
appropriate for the type of data that I collected because it reduced the number of dose-treatments
needed, allowed for the same batch of insects to be checked daily and accounted for censored data
(insects surviving beyond the time frame of the experiment).
Of the 30 studies surveyed included in table 4, 13 used a probit analysis, 8 a survival
analysis, 3 used both, and 6 used either another type of analysis or did not specify.
40
Table 4: A survey of experimental design and statistical methods used in 30 studies; selected from
a Google Scholer search with key words “Metarhizium + Bioassay”, limited to 2010-2014.
Time – Response
Method of analysis
Host Treatment method
Gao et al. (2013)
Survival analysis Bombyx mori Larvae immersed in 5 ×106 suspension for 1 min or injected
with 10µl of 106 conidia/ml. 15 insect (×3) checked every
12h.
Garza-Hernandez et al. (2013)
Survival analysis Aedes aegypti
Infection of mosquitos co-infected with virus. 25 adults exposed to filter paper impregnated with 1 × 10
8 conidia/ml.
Checked daily until all dead.
Goble et al. (2014)
Survival analysis Anoplophora glabripennis
For 36 individuals the ventral surfaces were pressed on to two agar plugs with conidia for 5 sec. Also, for 24 beetles were submerged for 10 sec in a 15ml suspension of 1 × 10
7
conidia/ml. Checked daily for 50 days.
Howard et al. (2010)
Survival analysis Anopheles gambiae
25 adult mosquitos were placed in a tube with netting that had been treated in a fungus. Checked daily until all fungal treated individuals died.
Jin et al. (2012) Method not specified
Locusta migratoria
Adults were either: dipped up to the head-thorax junction in a soybean-oil suspension containing 1×10
7 conidia/ml; or,
injected with 5 µl of a 1 × 106 conidia/ml in the haemocoel
cavity through. Twenty insect per rep, checked every 12h.
Lopes et al. (2013)
Survival analysis Cosmopolites sordidus
Adults were submerged in conidial treatment of 1 × 108
conidia/ml for 90 sec. Sixteen-eighteen insects per treatments, mortality assessed every other day for 14 or 16 days.
Orduno-Cruz et al. (2011)
Logistic regression
Metamasius spinolae
Twenty adults were immersed in 500ml suspension with 1 ×10
8 conidia/ml for 10 second. Checked for 41 days.
Peng et al. (2011)
Survival analysis Anoplophora glabripennis
Females exposed to fiber bands impregnated with fungi. Males held on conidia-covered surface for 30 seconds. Checked daily for 50 days.
Quinelato et al. (2012)
Probit analysis & non-parametric Kruskal–Wallis test
Rhipicephalus microplus
Larvae (~100/tube) were immersed in 1.2 × 108, 10
7, 10
6 and
105 conidia/ml suspensions for 3 min. The suspension was
absorbed out of test tube, mortality checked every 5 days for 30 days. Mortality was estimated as a percentage.
Quintela et al. (2013)
Probit analysis and Survival analysis
Tibraca limbativentris
Adults were inoculated with 10µl of 5 × 107 conidia/mL
suspension on the dorsal region. Checked daily for 12 days.
Reyes-Villanueva et al. (2011)
Survival analysis Aedes aegypti
Females exposed to filter paper impregnated with 6 × 108
conidia/ml for 48 hours and checked for survival. Also, females exposed to exposed males that had been exposed to impregnated filter paper for 48h and watched for survival.
San Andrés et al. (2014)
Probit analysis Ceratitis capitata
Adults exposed for 30s to an “infective dish”, a dish with 3.1 × 10
8 conidia spread uniformly over the dish. 10 host per
treatment checked daily for 10 days.
Tavassoli et al. (2012)
General linear model and repeated measure analysis
Ornithodoros lahorensis
Eggs, larvae, and adult ticks were immersed in either 1 × 105
or 1 × 107 conidia/ml for 5s. Survival was checked every 3
days for 21days.
Wang et al. (2012)
Survival analysis Bombyx mori & Locusta migratoria
Silkworms injected with 10 μL of suspension of 5 × 105
conidia/ml, locust injected with 10 µl of 1 × 107. Ten insects
in each repetition. Mortality checked every 12 hours.
Wang et al. (2014)
Probit analysis Galleria mellonella & Tenebrio molitor
Each individual larva (30 per repetition) was sprayed with 1 ml of suspension of 10
7 conidia/ml. Monitored daily for
mortality.
41
Dose – Response
Ansari et al. (2010)
Probit analysis Culicoides nubeculosus
Eggs suspended in 108 conidia/ml until hatch. Larvae
suspended in 104, 10
5, 10
6, 10
7, or 10
8 conidia/ml – checked
for 3 days.
Contreras et al. (2014)
Probit analysis Tuta absoluta Eight pupae suspended in one of six concentrations (0.34-11.15 × 10
9 viable conidia per liter), checked every 3 days
for up to 3 weeks.
Leemon and Jonsson (2012)
Probit analysis Rhipicephalus microplus & Lucilia cuprina
Six fungal concentrations ranging from 1 × 109 to
1 × 104 conidia/ml. Ticks were either topically inoculated with
2µl or submerged in inoculum. Blowflies were either topically treated with 2µl suspension or fungi was mixed with food source. 20 insects per treatment, checked for 10 days.
Luz et al. (2011)
Probit analysis Anopheles gambiae and A. arabiensis
Eggs were topically treated with 5 × 106 conidia/cm
2. Also,
eggs in soil treated with oil formulation of 105, 3.3 × 10
5, 10
6,
3.3 × 106, and 10
7 conidia/cm
2. Checked every 5 d for 30 d.
Nussenbaum and Lecuona (2012)
Probit analysis Anthonomus grandis
Lots of isolates tested by submerging adults for 15 sec in a 5 × 10
8 conidia/ml, checked daily for 20 d. Also, 40 individuals
immersed treatments of: 1 × 106, 5 × 10
6, 1 × 10
7, 5 × 10
7,
1 × 108 and 5 × 10
8 conidia/ml; checked daily for 15 d.
Zayed et al. (2013)
Probit analysis Phlebotomus papatasi
Suspension of 1 × 106, 5 × 10
6, 1 × 10
7, 5 × 10
7, 1 × 10
8, and
5 × 108 conidia/ml prepared. 0.5g of each was mixed with 0.15g finely ground larval diet. 10 larvae added to each vile. 9 replicates. Mortality based on failure for adult to emerge.
Behle and Jackson (2014)
Method not specified
Alphitobius diaperinus
Larvae were exposed to treated soil. Conidial treatment ranged from 1.69 × 10
7 to 2.08 × 10
5 conidia/ml. 30 larvae
per dosage was used. Mortality was monitored for 14 days.
Both Dose and Time Response
Jin et al. (2011) Method not specified
Nilaparvata lugens
Thirty-forty nymphs were sprayed at 5 different rates on with one of three fungal concentrations (2 × 10
8, 2 × 10
7 and 2 ×
106 conidia/mL). Checked daily.
Kirubakaran et al. (2013)
Probit analysis and ANOVA
Cnaphalocrocis medinalis
Leaves sprayed with 5ml of 1 × 103, 1 × 10
4, 1 × 10
5, 1 × 10
6,
1 × 107 and 1 × 10
8 conidia/ml in water or oil formulation, 20
larvae exposed to treatments, checked daily for 8 days.
Maldonado-Blanco et al. (2013)
Probit analysis Aedes aegypti Submersion of 25 larvae in fungal concentrations of 1 × 105,
3 × 105, 5 × 10
5, 8 × 10
5 or 1 × 10
6 submerged spores/ml.
Insects checked daily for 5 days.
Mishra et al. (2011)
Probit analysis Musca domestica
One ml fungal suspension of 103, 10
5, 10
6, 10
7, and
109 conidia/ml were applied to fly diet. Checked daily for 5
days. Also done in an arena setup.
Ortiz-Urquiza et al. (2013)
Probit analysis and Survival analysis
Ceratitis capitata & G. mellenella
Adult flies were treated with 1 of 6 spore concentrations from 10
3 - 10
8 conidia/ml by spraying. Galleria larvae treated by
injecting 8µl of suspension. 10 insect per treatment.
Shan and Feng (2010).
Method not specified
Myzus persicae A leaf with 40 adult aphids was sprayed with 1 ml suspension, 1 × 10
6, 1 × 10
7 and 1 × 10
8 conidia/ml),
mortality was checked daily for 8 days.
Vázquez-Martínez et al. (2013)
Probit analysis Anopheles albimanus
Larvae were placed in cups with 200 ml of 2.6×107
conidia/mL. Checked daily until dead or adult emergence. Adults were immobilized with cold and inoculated with 5µl 2.7×10
8 conidia/mL suspension. Checked daily for 7 days.
Yousef et al. (2013)
Probit analysis and Survival analysis
Bactrocera oleae
Adults were treated with 1 ml of a 1.0 × 108 conidia/ml by
spraying. Checked daily for 12 d. Two assays for puparia. 1. 1 ml of a10
8 conidia/ml added to 30g soil with 63 puparia; 2.
Puparia immersed in fungal suspension for 10 seconds.
42
v. Conclusion and future perspectives
The use of living organisms to control pest insects is an important part of current and future
crop protection. Understanding the fundamental ecology of these organisms is vital to their success
as BCAs. For example, research regarding their natural occurrence and effect on host populations
greatly enhances their potential for more efficient utilization in pest regulation; e.g., conservation
biological control. Additionally, research which investigates how these organisms interact with
other organisms, viz. plants, plant pathogens and other BCAs, is crucial to predicting their
effectiveness and maintaining consistency as BCAs. This thesis advances the current scientific
knowledge regarding the ecology and biological control use of Metarhizium spp. fungi in several
areas, namely:
M. flavoviride is the dominant species of the Metarhizium community found in some
agroecosystems in Denmark.
Significant intra-species diversity exists within the understudied species M. flavoviride.
M. brunneum, M. flavoviride and M. robertsii, applied as a seed treatment of conidia, will
disperse through soil with a growing plant root. Furthermore, these species of Metarhizium
will maintain pathogenicity to insects while interacting with plant roots.
Dual BCA seed treatments of C. rosea and M. brunneum or M. flavoviride will control F.
culmorum infection in wheat seedlings.
A reduction in virulence occurs when M. brunneum or M. flavoviride and C. rosea are
applied as a seed treatment on F. culmorum infected plants. However, virulence to T.
molitor was still observed at a significant level when compared to untreated controls.
Perhaps one of the most valuable components of any research is not the conclusion provided
but rather the new questions that remain unanswered. Based on the observations of this thesis there
are several research questions that I think should be addressed, including:
Worldwide survey studies that endeavor to elucidate the distribution and occurrence of
Metarhizium spp. in agriculture. These studies should emphasize habitat associations as
well seeking to understand what characteristics promote abundance in particular areas.
Highly important to these studies will be the continued development of molecularly based
ecological tools, like isolating SSR markers (microsatellites) that can explicitly discriminate
genotypic diversity within the M. flavoviride species.
43
Field studies to evaluate the effectiveness of Metarhizium seed treatment in protecting crops
from pest insects. These studies will not only evaluate infectivity, but also the longevity of
fungal survival in field, and effects of crop type.
Investigation into the mechanisms that resulted in reduced virulence when Metarhizium was
co-treated with another fungus. This study will investigate both direct interactions such as
antifungal metabolite production and mycoparasitism, as well as indirect interaction such as
resource competition.
Additional studies into the synergistic or combined effects of using multiple BCA to control
different plant pests and disease. There was some indication that Metarhizium spp.,
especially M. flavoviride, has antifungal properties; however, no control of F. culmorum
disease was observed on the plant. Effects may be realized with different treatment
methods, plant types or fungal concentrations.
44
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vii. Appendix
Manuscript 1
METARHIZIUM SEED TREATMENT MEDIATES FUNGAL DISPERSAL VIA ROOTS AND INDUCES
INFECTIONS IN INSECTS
Chad A. Keyser, Kristian Thorup-Kristensen, & Nicolai V. Meyling
Status: Published in Fungal Eclology, October 2014, Vol. 11, pg. 122-131
Printed version reproduced with permission from Elsevier – License Number: 3531750730534
Metarhizium seed treatment mediates fungaldispersal via roots and induces infections in insects
Chad A. KEYSERa,*, Kristian THORUP-KRISTENSENb, Nicolai V. MEYLINGa
aDepartment of Plant and Environmental Sciences, University of Copenhagen, Thorvaldsensvej 40,
1871 Frederiksberg, DenmarkbDepartment of Plant and Environmental Sciences, University of Copenhagen, Hojbakkeg�ard Alle 13,
2630 Taastrup, Denmark
a r t i c l e i n f o
Article history:
Received 28 March 2014
Revision received 1 May 2014
Accepted 5 May 2014
Available online
Corresponding editor:
Duur Aanen
Keywords:
Below ground interactions
Biological control
Entomopathogenic fungi
Plant protection
a b s t r a c t
The study aimed to evaluate the extent to which Metarhizium spp. applied as conidia to
seeds will disperse with the growing root system and maintain pathogenicity after dis-
persion. Tenebrio molitor larvae were exposed to roots of wheat plants that had been grown
from seeds inoculated with conidia of either M. brunneum (KVL 04-57 and KVL 12-37) or M.
robertsii (ARSEF 2575 and KVL 12-35) in both laboratory and greenhouse settings. All four
Metarhizium isolates tested maintained pathogenicity towards T. molitor larvae for up to 4
weeks after being dispersed by roots through both an artificial growth substratum and non-
sterile soil. Based on these results we propose that a planteroot association benefits
entomopathogenic fungi with mobility in the soil and an increased likelihood of encoun-
tering a susceptible insect host.
ª 2014 Elsevier Ltd and The British Mycological Society. All rights reserved.
Introduction
The soil-inhabiting mitosporic entomopathogenic fungal
genus Metarhizium (Hypocreales: Clavicipitaceae) has a cos-
mopolitan distribution and a wide range of arthropod hosts
(Zimmermann, 2007). As early as 1888 the potential for a
biological control agentwas recognized and aMetarhizium spp.
isolate wasmass produced and applied to control a pest insect
(Krassilstschik, 1888; Roberts and St. Leger, 2004). Both the
need and hope for a reliable biological control agent have
fueled Metarhizium research for more than a century.
Emphasis placed on developing a biological control agent has,
however, resulted in a neglect of research concerning basic
Metarhizium ecology which may be essential to its success for
biological control (Bruck, 2005; Meyling and Eilenberg, 2007;
Vega et al., 2009).
To fill this gap of knowledge, several studies have recently
focused on the fundamental ecology of these fungi both in
their natural habitats and in the ecosystems where they are
applied. These have shown that genotypic groups of Meta-
rhizium spp. can associate closely with habitat and plant
species (Bidochka et al., 2001; Fisher et al., 2011; Wyrebek
et al., 2011). Rhizosphere competence, the ability of a micro-
organism to proliferate and function in the rhizosphere
* Corresponding author. Department of Plant and Environmental Sciences, University of Copenhagen, Thorvaldsensvej 40, Stair 2, 3rdFloor, B321, 1871 Frederiksberg, Denmark.
E-mail address: [email protected] (C.A. Keyser).
available at www.sciencedirect.com
ScienceDirect
journal homepage: www.elsevier .com/locate/ funeco
http://dx.doi.org/10.1016/j.funeco.2014.05.0051754-5048/ª 2014 Elsevier Ltd and The British Mycological Society. All rights reserved.
f u n g a l e c o l o g y 1 1 ( 2 0 1 4 ) 1 2 2e1 3 1
(St Leger, 2008), was observed in Metarhizium spp. isolates
(Bruck, 2005; Hu and St Leger, 2002). Furthermore,Metarhizium
spp. applied to the rhizosphere have been shown to benefit
plant growth and aid in plant-nutrient acquisition (Behie and
Bidochka, 2014; Behie et al., 2012; Khan et al., 2012; Sasan and
Bidochka, 2012), and it is now clear that the ecological com-
plexity and importance of the fungal genus Metarhizium
extend beyond that of ‘entomopathogen’.
One central question that remains to be explored is what
benefitsMetarhizium derives from plant associations. Thus far
the focus of endophytic interaction between plants and Met-
arhizium has been characterized by how the plant has bene-
fitted, eg. through nutrient acquisition (Behie et al., 2012),
while if and how the fungus benefits have largely been
ignored. Metarhizium spp. can process and utilize plant-
derived carbohydrates available in the rhizosphere for
growth (Fang and St Leger, 2010; Pava-Ripoll et al., 2011) but it
is possible that Metarhizium spp. acting as plant symbionts
might also increase their exposure to prospective host insects.
For example, actively growing plant roots could provide non-
mobile microorganisms, such as Metarhizium spp. with a
means of dispersal, thus increasing their chance of finding a
host insect. It can be assumed that there is an increased
likelihood of encountering a root feeding herbivore near its
food source (Park and Tollefson, 2005; Prystupa et al., 1988).
The first step towards answering these questions is to
determine if Metarhizium retains its pathogenicity while
associating with plant roots. Bruck (2005) found that root
cuttings inoculated with Metarhizium conidia (actually M.
brunneum) resulted in successful infections of root feeding
black vine weevil (Otiorhynchus sulcatus) larvae. Kabaluk and
Ericsson (2007) discovered Metarhizium infected wire worm
larvae (Agriotes obscurus) after sowing Metarhizium-treated (M.
brunneum) corn seeds in a field trial. They also observed an
increased yield in corn production when the seeds were
treated with the fungus and speculated that the observed
yield increase was due to seedlings being protected from
insect attack either by insects being infected or repelled by the
fungus. However, further studies are needed to determine the
effectiveness of seed treatments in infecting insects.
The hypothesis tested in this study was that Metarhizium
spp. applied as seed treatment will disperse with roots in non-
sterile soil and retain the ability to infect insects. To test this
hypothesis, Tenebrio molitor larvaewere exposed to the roots of
wheat plants that had been grown from seeds inoculated with
Metarhizium spp. conidia in both laboratory and greenhouse
settings. In addition a traditional infection bioassay was per-
formed to determine the virulence of the fungal isolates
included in this study.
Materials and methods
Fungal preparation
Four isolates of Metarhizium spp. were included in this study.
Two isolates ofM. robertsii (Mr): ARSEF 2575 obtained from the
USDA-ARS Collection of Entomopathogenic Fungal Cultures
(ARSEF) (USDA Plant, Soil and Nutrition Laboratory, Ithaca,
NY, USA) and KVL 12-35, isolated from agricultural soil in
Denmark (Steinwender, 2013); and two isolates ofM. brunneum
(Mb): KVL 04-57, same genotype as the active ingredient of the
commercial isolate Met52 (Novozymes, Salam, Virginia), and
KVL 12-37, isolated from agricultural soil in Denmark
(Steinwender, 2013). All four isolates are maintained at �80 �Cat the University of Copenhagen andwere identified to species
using DNA sequencing following Bischoff et al. (2009).
Fresh cultures of each isolate were prepared for experi-
ments from a stock culture, each grown for 2e3 weeks on
Sabouraud Dextrose Agar (SDA) (Merck KGaA, Darmstadt,
Germany) at 26 �C. Conidia were then harvested with a sterile
spatula and suspended in 0.005 % Triton X-100 (Sigma
Chemical, MO, USA), the suspension was then passed
through glass wool to remove hyphae, conidial clumps and
loose agar. Each suspension was vortexed and conidial con-
centrations estimated by counting in a hemocytometer
(Fuchs-Rosenthal).
Conidial viability was checked by transferring 20 ml of the
suspension onto agar medium [4-ml SDA with 0.002 %
Benomyl active ingredient (SigmaeAldrich, MO, USA)] and
counting conidia germination after 48 hr at 26 �C; suspensionswere only used if germination was greater than 90 %.
Seed treatment assay
Seed treatmentsFor each isolate of Metarhizium a 1 � 108 conidia ml�1 sus-
pension was prepared and then diluted to create a second
suspension of 1 � 107 conidia ml�1. Wheat seeds (Triticum
aestivum) were pre-germinated to ensure viability and then
soaked for 1 hr in a fungal treatment or distilled water (con-
trol); they were then removed and allowed to dry on filter
paper at room temperature. A prescreening of several vari-
eties ofwheat indicated that surface sterilizing seeds removed
some but not all natural occurrence ofmicrobes; tomaintain a
realistic seed-borne microbial community the wheat seeds
were not surface sterilized.
Paper roll setupTen treated seeds were evenly spaced 2 cm from the top edge
of 2-ply filter paper (58 � 29 cm) (Frisenette ApS, Denmark)
which had been moistened to saturation with ddH2O. Seeds
were then secured by placing a strip of filter paper (7 � 58 cm)
along the top of the paper, whichwas rolled up into a tube and
placed standing upright with seeds in the top in a 600 ml
beaker with 200 ml ddH20, placing the seed approx. 22 cm
from the surface of thewater (Supplementary Fig S1). Each roll
was wrapped in a piece of aluminum foil to keep seeds in the
dark and reduce evaporation and then placed under a growth
lamp with 12/12 hr light/dark regime at room temperature
(21 �C � 2) for 14 d. The resulting data from this setup will be
referred to as either Paper 108 or Paper 107 according to the
spore concentration. The setup was repeated on four separate
occasions.
Soil-pot experimentIn the greenhouse, pots were prepared with sandy non-sterile
subsoil taken from the lower horizon (20e60 cm) of an Agru-
dalf soil at the University research farm in Taastrup, Den-
mark. The texture of the soil was 3.9 % clay, 4.7 % silt, 33.3 %
Metarhizium dispersal via roots 123
fine sand, 57.1 % coarse sand and 1 % humus. Forty treated
seeds were distributed over the surface of the soil in each pot
and allowed to grow in a greenhouse at 20 �C day/15 �C night
temperature regime with 12/12 hr light/dark. The soil was
screened for entomopathogenic fungi before the experiment
using insect baiting and plating suspensions on selective
media [CTC media (Fernandes et al., 2010) amended with
0.02 g dodine (Agriphar, Belgium)]. No Metarhizium or other
entomopathogenic fungal taxa were recovered, suggesting
that naturally occurring Metarhizium spp. should not be
expected in the experimental soil used. Roots, from the same
growing pot, were harvested at 2 and 4 weeks after planting
(w20 randomly selected plants per harvest) by gently remov-
ing the plant from the soil and shaking off loose soil. Roots
were placed in 50 ml centrifuge tubes and kept at 5 �C until
they were used for the bioassay the following day. The data
resulting from this setupwill be labeled: Pot2w 108, Pot2w 107,
Pot4w 108 or Pot4w 107 according to the time of harvest and
spore concentration. The setup was repeated on four separate
occasions.
Root/insect assayPetri plates (60 � 15 with vents, Greenbio One, Hungary) were
lined with a single sheet of filter paper (Size 55, VWR inter-
national, France) and moistened with 200 ml of ddH20. For
roots from the potted plants 0.2e0.3 g of root material was cut
2 cm below the seed, washed with distilled water to remove
loose soil, and added to each Petri plate (three replicate plates
per treatment were prepared). For root material from the
paper roll setup, 0.1e0.2 g of root material was cut 2 cm below
the seed and added to a Petri plate (three replicates per
treatment). These root portions were representative of a plant
root system starting 2 cm below the seed and extending
w10 cm down for a single plant, however, root material used
for the experiment consisted of several root laterals randomly
selected from different plants of the same harvest. After
adding the cut-root section to each Petri plate ten T. molitor
(Coleoptera: Tenebrionidae) larvae (Avifauna, Copenhagen,
Denmark) were added to each Petri plate. Further, a Petri plate
with 10 T. molitor larvae was prepared with 10e14 g of soil
collected from the potted plants setup, the soil was collected
immediately after the roots were harvested. All plates with
larvae were checked regularly and any dead insects were
removed, washed in ddH2O and placed separately in medicine
cups to check for mycosis.
Additionally a sample of root (of the sameweight as used in
the insect assay) was cut from each treatment group (those
originating from the potted plants were washed), homogen-
ized in 5 ml of ddH20, and 200 ml of this homogenate was
pipetted on to selective media (see above) and incubated for 2
weeks at 22 �C. Metarhizium colonies were identified and the
number of colony forming units (CFUs) assessed.
These procedures were repeated four times with the two
experimental setups on different weeks using new fungal
cultures, soil, seeds and insects.
Virulence bioassay
For each of the four isolates of Metarhizium spp. a
1 � 107 conidia ml�1 suspension was prepared and then serial
diluted to prepare a 1 � 104 conidia ml�1 suspension. As in
the Root/insect assay experiment, three Petri plates of ten
larvae (with moistened filter paper) were prepared for each
fungal treatment plus two controls (the two controls are
exactly the same and the results were combined for the
analysis). Ten T. molitor larvae were individually treated with
5 ml of the designated suspension by pipette and placed
together in a single Petri plate (30 treated larvae per treat-
ment). The Petri plates were then stacked as a treatment
group, secured with an elastic band and placed in a plastic
box with moist paper towels on the bottom to maintain high
humidity. The treated insects were then incubated at 26 �C in
the dark. Mortality was checked daily, dead insects were
removed and surface sterilized by dipping each cadaver for
2 s in 70 % ethanol, 2 s in 7e5 % sodium hypochlorite and
then rinsed three times in ddH2O. The cadavers were then
placed in medicine cups with moist filter paper in order to
observe mycosis. The infection bioassays were repeated
three times on different weeks with new fungal cultures and
insects. This study will be referred to as Bioassay 107 or
Bioassay 104 depending on dilution.
Statistical analysis
Mortality and mycosis data from the root/insect assay
experiment were analyzed using a mixed model (with nlme
library for R) with the fungal isolate as the effects factor and
trial as the random factor. Prior to the analysis, data were split
into groups according to growth conditions, harvest time
and fungal dose (Paper 108, Paper 107, Pot2w 108, Pot2w 107,
Pot4w 108 or Pot4w 107) and analyzed separately. Assump-
tions of normality and homogeneity were met without
transformations.
A Pearson correlation analysis was performed with the
root/insect assaymortality ormycosis data and the CFUs from
root homogenate plated on selective media. The analysis was
performed in RStudio (version 0.97.551) using the cor.test
procedure.
For the virulence bioassay, mortality of the fungal isolate
treatments relative to the control were calculated as hazard
ratios (HR; relative average daily risk of death) fit to the sur-
vival data using a mixed Cox Proportional Hazards (PH)
regression model (Cox, 1972). The Cox PH model is based on
the assumption that while the risk of death is different from
one group to another, it remains constantly proportional over
time. This proportion is expressed as the hazard ratio, where
a value of 1.0 indicates that the two treatments have the
same risk of death at any given time. Pairwise comparisons
between the fungal treatments were performed by setting
each isolate as the reference group in the mixed model and
generating HR values. The risk of death of one treatment was
considered significantly different from another if the p-value
was less than 0.01 (0.05 divided by five pairwise compar-
isons). These analyses were performed in Rstudio using the
coxme package.
Post-hoc comparisons for both the virulence bioassay sur-
vival data and the root/insect assay data were performed
using the ghlt function in the multcomp package for R. P-
values less than 0.05 were considered significant. All of the
analyses were performed in RStudio (version 0.97.551).
124 C.A. Keyser et al.
Results
Seed treatment assay
Paper rollsA significant effect of fungal seed treatment on T. molitor
larvae mortality after exposure to washed roots 14 d after
inoculation was observed in both Paper 107 and Paper 108
experiments (F ¼ 7.4, df ¼ 4, p < 0.0001, F ¼ 12.5, df ¼ 4,
p < 0.0001, respectively; Fig 1) with higher mortalities in
fungal treatments than controls except for isolate KVL 12-37
(Mb) in Paper 107 (Fig 1A). No mycosis was observed in the
dead insects from the control treatments (Table 1). For
mycosis a significant effect of fungal treatment was noted in
both Paper 107 and Paper 108 (F ¼ 5.5, df ¼ 4, p ¼ 0.0007,
F ¼ 11.6, df ¼ 4, p < 0.0001, respectively). In Paper 108 sig-
nificantly more mycosis than in the control was observed in
all isolates except ARSEF 2575 (Mr); while for Paper 107 only
KVL 04-57 (Mb) had significantly more mycosis than the
control (Table 1). It is noteworthy, however, that many of
the dead insects from the fungal-treated groups showed
signs of fungal infection (melanization spots on the cuticle;
C.A. Keyser, pers. obs.) but fungi did not emerge from
cadavers.
Soil-pot assayTwo weeks after planting, the effect of fungal treatment on
larval mortality for Pot2w 107 was not significant (F ¼ 2.4,
df ¼ 4, p ¼ 0.06) despite all of the fungal treatments resulting
in mean mortalities apparently higher than in the control
(Fig 2A). Larvae exposed to soil collected from the pots with
wheat plants grown from seed inoculated with
107 conidia ml�1 showed significant effect of treatment
(F ¼ 3.05, df ¼ 4, p ¼ 0.04), but only KVL 12-37 (Mb) showed
significantly higher mortality than the control (Fig 2B). For
Pot2w 108 a significant effect of fungal treatment was found
(F ¼ 5.5, df ¼ 4, p ¼ 0.0007); T. molitor larvae exposed to roots
grown from wheat seeds treated with either of the Danish
isolates [KVL 12-35 (Mr) and KVL 12-37 (Mb)] had significantly
higher mortality than the control (Fig 2C). Mortality of larvae
placed with soil from the same experiment was also sig-
nificantly affected by treatment (F ¼ 5.92, df ¼ 4, p ¼ 0.004)
with higher mortalities for both M. brunneum isolates and M.
robertsii isolate KVL 12-35 (Fig 2D). No mycosis was observed
in any of the control treatment groups for larvae exposed to
either roots or soil (Table 1); the effect of fungal treatment on
mycosis was significant for both larvae exposed to roots and
soil at the low and high doses (F ¼ 5.36, df ¼ 4, p ¼ 0.0011;
F ¼ 3.02, df ¼ 4, p ¼ 0.049; F ¼ 6.95, df ¼ 4, p ¼ 0.0001; F ¼ 6.95,
df ¼ 4, p ¼ 0.0019, respectively).
After 4 weeks of plant growth a significant effect of fungal
treatment for Pot4w 107 on mortality was observed when
larvae were exposed to washed roots (F ¼ 3.4, df ¼ 4, p ¼ 0.01).
Both isolates KVL 12-35 (Mr) and KVL 04-57 (Mb) showed sig-
nificantly more mortality than the control (Fig 3A). In the soil
experiment, the effect of fungal treatment was almost sig-
nificant (F ¼ 2.9, df ¼ 4, p ¼ 0.05) with KVL 04-57 (Mb) causing
higher mortality than the control (Fig 3B). For the Pot4w 108
experiment a significant effect was observed among the
fungal treatments (F ¼ 8.7, df ¼ 4, p < 0.0001) where KVL 12-35
(Mr) and KVL 04-57 (Mb) showed higher mortality than the
control (Fig 3C). In the soil treatment all of the fungal isolates
caused higher mortality than the control (F ¼ 8.46, df ¼ 4,
p > 0.0001; Fig 3D). Mycosis was not detected in any of the
control treatment groups for larvae exposed to either roots or
soil after 4 weeks (Table 1). The effect of fungal treatment on
mycosis was significant for both larvae exposed to roots at
low and high dose and soil at the high dose (F ¼ 2.96, df ¼ 4,
p ¼ 0.026; F ¼ 9.65, df ¼ 4, p < 0.0001; F ¼ 10.42, df ¼ 4,
p < 0.0001, respectively); no significant effect was observed
Fig 1 e Mean percent mortality (DSE) of T. molitor larvae
after exposure to roots of wheat plant grown from
Metahizium inoculated seeds for 14 d. Seeds were
inoculated by soaking for 1 hr in suspensions of either
1 3 107 (A) or 1 3 108 (B) conidia mlL1 or water (control).
Mortality was based on 30 larvae per treatment and each
treatment was repeated four times. Different letters on
bars indicate significant differences within each treatment
group.
Metarhizium dispersal via roots 125
for mycosis in the soil at the low dose (F ¼ 2.21, df ¼ 4,
p ¼ 0.112).
CFU counts on plates correlationsNo Metarhizium CFUs were observed on the root homogenates
from control plants when plated on selective media. Positive
correlations between the number of CFUs on selective media
and the mortality in the root/insect assay (Pearson r ¼ 0.38,
df ¼ 88, p ¼ 0.0002) and between CFUs and mycosis was
observed (Pearson r ¼ 0.42, df ¼ 88, p < 0.0001; data not
shown).
Virulence assay
A significant effect of treatment was observed in both Bio-
assay 107 and Bioassay 104 (c2 ¼ 641.84, df ¼ 4, p < 0.0001;
c2 ¼ 123.14, df ¼ 4, p < 0.0001, respectively). Higher mortality
was observed among all larvae treated with a fungal isolate as
compared to control treatments in both Bioassay 107 and
Bioassay 104 (HR ¼ 100.45, p < 0.001 and HR ¼ 5.8, p < 0.001,
respectively). The median survival time for the four fungal
treatments for Bioassay 107 was 5 d (Fig 4A); however, isolate
KVL 12-37 (Mb) was significantly less virulent than the other
isolates (Fig 4B). For Bioassay 104 the median survival time
could only be established for KVL 04-57 (Mb) for which it was
14 d while the other fungal treatments did not cause 50 %
mortality within the course of the experiment (Fig 4C). How-
ever, all of the fungal treatments were more virulent than the
control; KVL 04-57 (Mb) was statistically the most virulent
(Fig 4D).
No mycosis of Metarhizium was detected on insects from
the control group. Mycosis was observed on dead larvae from
all four fungal-treated groups (Table 2). Significantly more
mycosis was observed on larvae from Bioassay 107 than Bio-
assay 104 (F ¼ 20.31, df ¼ 1, p < 0.0001). For both Bioassay 104
and Bioassay 107 the effect of treatment on mycosis was
significant (F ¼ 23.6, df ¼ 4, p < 0.0001; F ¼ 165.1, df ¼ 4,
p < 0.0001, respectively).
Discussion
All of the Metarhizium isolates tested in this study maintained
pathogenicity towards T. molitor larvae after being dispersed
by roots through both an artificial growth substratum and
non-sterile soil. The ability of seed-treated Metarhizium to
disperse through soil via a root system is highly relevant for
biological control programs. Bruck (2005) stated that “by
developing techniques to use the roots as a delivery system for
entomopathogenic fungi, the cost and logistics of biological
control would be much more favorable”. In the current study
the relatively small quantity of conidia applied to each seed
was sufficient to inoculate both the washed root and the
surrounding soil with sufficient Metarhizium propagules to
initiate lethal infections.
In the experiment Bioassay 104, M. brunneum KVL 04-57
was the most virulent isolate tested. Several studies have
shown that the commercial product Met52 (¼F52), the same
genotype as KVL 04-57, has good efficacy against a wide range
of soil-dwelling insect pests (Bruck et al., 2005; Liu and Bauer,
2006; Jaronski and Jackson, 2008; Ansari and Butt, 2013).
However, in this study, none of the isolates were consistently
more virulent when applied as a seed treatment. Foster et al.
(2010) also observed that in laboratory studies the F52 strain
was highly virulent, however, in field trials the effectiveness
was reduced. While virulence observed in the laboratory is a
useful trait when comparing isolates it often does not trans-
late to field efficacy. The present results demonstrated that
isolates retained their pathogenicity even in non-sterile soil,
suggesting that fungal presence can potentially protect roots
from damage by herbivores.
CFU counts from the homogenized root samples indicated
that, for all three 108 conidia ml�1 root assays (Paper 108,
Pot2w 108, and Pot4w 108), the infection dose supplied to each
Petri dish of T. molitor larvae was equal to that administered to
the insects in Bioassay 104 (w500 propagules/10 larvae).
Although the results are not directly comparable, in Bioassay
104 the averagemortality ranged from 26 to 62% after 2weeks.
Table 1eMeanpercent of observedmycosis (±SE) byMetarhizium spp. among dead T.molitor larvae after exposure towheatroots or soil for 14 d. The seeds were grown in one of three conditions: paper rolls for 2 weeks, soil pots for 2 weeks, or soilpots for 4 weeks. Letters designate significant differences within column and treatment conditions
2 weeks 4 weeks
Paper Roots from soil Soil Roots from soil Soil
1 3 107 conidia mlL1
Control 0.0a 0.0a 0.0a 0.0a 0.0a
ARSEF 2575 (Mr) 9.2(�4.8)a 0.0(�0.0)ab 7.5(�7.5)ab 1.7(�1.7)a 25(�25.0)ab
KVL 12-35 (Mr) 15.0(�5.2)ab 8.3(�5.5)b 20(�11.5)ab 11.7(�6.7)b 20(�20.0)ab
KVL 12-37 (Mb) 9.2(�7.1)a 2.5(�2.5)ab 22.5(�14.3)b 0.0(�0.0)a 12.5(�7.5)ab
KVL 04-57 (Mb) 30.8(�17.1)b 8.3(�3.5)b 10(�5.7)ab 7.5(�5.5)ab 52.5(�21.3)b
1 3 108 conidia mlL1
Control 0.0a 0.0a 0.0a 0.0a 0.0a
ARSEF 2575 (Mr) 8.3(�7.3)ab 1.7(�1.7)ab 10(�10)ab 0.0(�0.0)a 37.5(�22.5)ab
KVL 12-35 (Mr) 32.5(�14.1)bc 31.7(�21.8)c 77.5(�16.5)c 46.7(�19.8)b 92.5(�4.7)c
KVL 12-37 (Mb) 29.2(�7.6)bc 20.8(�14.2)bc 37.5(�22.5)abc 20.8(�15.8)b 47.5(�15.4)bc
KVL 04-57 (Mb) 49.2(�3.7)c 3.3(�3.3)ab 55(�21.0)bc 29.2(�13.7)b 72.5(�24.2)bc
126 C.A. Keyser et al.
In Pot4w 108 the average mortality similarly ranged between
16 and 54 % after 2 weeks exposure to roots. These data
indicate that despite the complexity of the growing conditions
during the 4 weeks in non-sterile soil in greenhouse settings
(e.g., variable temperature, fluctuating moisture levels, com-
petition with other microorganism for resources, etc.), path-
ogenicity was not obviated in the soil.
Nitrogen acquisition by plants from an otherwise
unavailable source (insects) has been demonstrated as a result
of association with several entomopathogenic fungal species
(Behie et al., 2012; Behie and Bidochka, 2014) obviously to the
benefit for the plant. It is likely that the funguswill also benefit
from this association, and Metarhizium spp. have been shown
to grow in root exudate (Fang and St Leger, 2010; Pava-Ripoll
et al., 2011), suggesting that it is likely that the fungus profits
from the carbohydrate rich environment in the rhizosphere to
buildup biomass. However, we expect that the fungus ulti-
mately benefits from the association with the root by being
able to locate and infect new insect hosts where buildup of
biomass and infective units, i.e., conidia, is likely to be much
greater than in the rhizosphere. Since soil-dwelling insects are
likely to be more abundant in the nutrient rich rhizosphere
Fig 2 e Mean percent mortality (DSE) of T. molitor larvae after exposure to roots of wheat plants grown from Metarhizium
inoculated seeds (Roots) or experimental soil (Soil) for 14 d. Roots and soil were collected 14 d after planting. Seeds were
inoculated by soaking for 1 hr in suspensions of either 1 3 107 (A and B) or 1 3 108 (C and D) conidia mlL1 or water (control).
Mortality was based on 30 larvae per treatment and each treatment was repeated four times. Different letters on bars
indicate significant differences within each treatment group.
Metarhizium dispersal via roots 127
than elsewhere in the soil (Walker et al., 2003) the root asso-
ciation of Metarhizium can be regarded as a vehicle to
encounter suitable insect hosts by an otherwise immobile
entomopathogen.
In general, dispersion of hypocrealean fungi is limited and
largely depends on passive dispersal by abiotic means such as
wind or rain (Meyling and Eilenberg, 2007). One of the benefits
a root-associating fungus derives from the plant interaction is
thus below ground mobility. This study clearly demonstrated
that infectious Metarhizium material was dispersed by roots.
Future studies evaluating both the effects on the plant and the
fungus would be particularly interesting and helpful in
determining if the rootefungus interaction should be con-
sidered as mutualistic. Dispersal by roots has been shown for
othermicroorganisms aswell, while percolatingwater is often
an important factor in ground dispersal it is noted that root
systems are either vital to, or greatly improve dispersal
(Bashan and Levanony, 1987; Elsas et al., 1991; Liddell and
Parke, 1989; Trevors et al., 1990). In the current study it is
important to note that the traditional watering system
employed in the greenhouse-pot experiment possibly aided
fungal dispersal, however, in the paper roll study moisture
was from below the growing plant. A further advantage of the
system utilized in this study is that it provides a platform to
A B
C D
Fig 3 e Mean percent mortality (DSE) of T. molitor larvae after exposure to roots of wheat plant grown from Metarhizium
inoculated seeds (Roots) or experimental soil (Soil) for 14 d. Seeds were inoculated by soaking for 1 hr in suspensions of
either 13 107 (A) and (B) or 13 108 (C) and (D) conidia mlL1 or water (control). Mortality was based on 30 larvae per treatment
and each treatment was repeated four times. Different letters on bars indicate significant differences within each treatment
group.
128 C.A. Keyser et al.
screen entomopathogens for effectiveness. While none of the
four isolates tested in the present plant interaction studies
were consistently more virulent than the others, the potential
to compare isolates to each other in a more realistic and
complex setting than a typical infection bioassay is evident.
Effective and cost efficient biological control agents such as
Metarhizium are an important aspect of current and future pest
management practices. A concerted effort to improve the
ecological understanding of these fungi will both improve
efficient application (e.g., seed treatments vs. field cover) and
ensure responsible usage. While much is still unknown, it is
clear thatMetarhizium spp. play both a complex and important
ecological role in the environment. The holdover paradigm,
from conventional pesticide practices, of only considering the
host/pathogen relationship is too limited in a biological con-
trol context. Wemust continue to increase our understanding
of the interactions between the biocontrol agent and themany
other organisms in those systems; such as, the plants we
intend them to protect, naturally occurring biota, and other
Fig 4 e Infection bioassay with four strains of Metarhizium. Mean survival of T. molitor larvae over 14 d after treatment with
5 ml of triton X (control) or a fungal suspension of either 1 3 107 or 1 3 104 conidia mlL1 (A, C). Pairwise comparisons of all
treatments within dose were determined using cox PHmodel and hazard ratios (relative risk of death) were calculated (B, D).
Values within each box indicate hazard ratios of the treatment on the y-axis in comparison to the treatment on the x-axis.
Two treatments that share a black square have a hazard ratio in relation to each other that is significantly different (D or L)
from one.
Table 2 e Mean percent of observed mycosis (±SE) byMetarhizium spp. among dead T. molitor larvae. Larvaewere treated with 5 ml of Triton X (control) or a fungaltreatment of either 1 3 104 or 1 3 107 conidia mlL1.Different letters designate significant differences withintreatment dose
Bioassay 104 Mycosis
Control 0(�0.0)a
ARSEF 2575 (Mr) 16.1(�16.2)a
KVL 12-35 (Mr) 68.3(�25.2)b
KVL 12-37 (Mb) 71.3(�20.0)b
KVL 04-57 (Mb) 83.4(�12.3)b
Bioassay 107 Mycosis
Control 0(�0.0)a
ARSEF 2575 (Mr) 84.4(�16.9)b
KVL 12-35 (Mr) 98.9(�1.9)b
KVL 12-37 (Mb) 94.4(�4.2)b
KVL 04-57 (Mb) 93.3(�4.1)b
applied biological agents e.g., predators, parasitoids, or
antagonists of plant pathogens.
Acknowledgments
We would like to give thanks to Jesper Andersen, Azmi Mah-
mood and Louise Lee Munk Larsen for their technical assis-
tance in this study and to Dr. Bernhardt M. Steinwender for
fruitful discussions. We also express gratitude to Richard
Humber for sending us several fungal cultures from the ARSEF
collection. This research was funded by a PhD grant to C.A.K
from the Plant Biosystems Elite Environment at the University
of Copenhagen.
Supplementary data
Supplementary data related to this article can be found at
http://dx.doi.org/10.1016/j.funeco.2014.05.005.
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Foster, R.N., Jaronski, S., Reuter, K.C., Black, L.R.,Schlothauer, R., 2010. Explaining mycoinsecticide activity:poor performance of spray and bait formulations of Beauveriabassiana and Metarhizium brunneum against Mormon cricketin field cage studies. Journal of Orthoptera Research 19 (2),303e313.
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Kabaluk, J.T., Ericsson, J.D., 2007. Metarhizium anisopliae seedtreatment increases yield of field corn when applied forwireworm control. Agronomy Journal 99 (5), 1377e1381.
Khan, A.L., Hamayun, M., Khan, S.A., Kang, S.M., Shinwari, Z.K.,Kamran, M., Lee, I.J., 2012. Pure culture of Metarhiziumanisopliae LHL07 reprograms soybean to higher growth andmitigates salt stress. World Journal of Microbiology andBiotechnology 28 (4), 1483e1494.
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Liu, H.P., Bauer, L.S., 2006. Susceptibility of Agrilus planipennis(Coleoptera : Buprestidae) to Beauveria bassiana andMetarhizium anisopliae. Journal of Economic Entomology 99 (4),1096e1103.
Meyling, N.V., Eilenberg, J., 2007. Ecology of theentomopathogenic fungi Beauveria bassiana and Metarhiziumanisopliae in temperate agroecosystems: potential forconservation biological control. Biological Control 43 (2),145e155.
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Pava-Ripoll, M., Angelini, C., Fang, W.G., Wang, S.B., Posada, F.J.,St Leger, R., 2011. The rhizosphere-competententomopathogen Metarhizium anisopliae expresses a specificsubset of genes in plant root exudate. Microbiology-SGM 157,47e55.
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Metarhizium dispersal via roots 131
63
Manuscript 2
BEST OF BOTH WORLDS: DUAL EFFECTS OF METARHIZIUM SPP. AND CLONOSTACHYS ROSEA
AGAINST AN INSECT AND A SEED BORNE PATHOGEN IN WHEAT
Chad A. Keyser, Birgit Jensen & Nicolai V. Meyling
Status: Under Review - Pest Management Science, submitted 22 Dec, 2014
64
Best of both worlds: Dual effects of Metarhizium spp. and Clonostachys rosea against an insect
and a seed borne pathogen in wheat
Chad A. Keyser1*, Birgit Jensen
2, and Nicolai V. Meyling
1
1Department of Plant and Environmental Sciences, Section for Organismal Biology, University of
Copenhagen, Thorvaldsensvej 40, 1871 Frederiksberg, Denmark
2Department of Plant and Environmental Sciences, Section for Genetics and Microbiology,
University of Copenhagen, Thorvaldsensvej 40, 1871 Frederiksberg, Denmark
*Corresponding author: Chad A. Keyser, Department of Plant and Environmental Sciences,
University of Copenhagen, Thorvaldsensvej 40,
1871 Frederiksberg, Denmark
Email: [email protected]
Running title
Dual effects of Metarhizium spp. and Clonostachys rosea
Keywords
Seed treatment; biological control, Fusarium culmorum, entomopathogenic fungi, mycoparasite
SUBMITED: PEST MANAGEMENT SCIENCE – 22 December 2014
65
Abstract
BACKGROUND: Crops are often prone to both insect herbivory and disease which necessitate
multiple control measures. Ideally an efficacious biological control agent must adequately control
the target organism and not be inhibited by other biological control agents when applied
simultaneously. Wheat seeds infected with the plant pathogen Fusarium culmorum were treated
with Metarhizium brunneum or M. flavoviride and Clonostachys rosea individually and in
combination with the expectation to control both root-feeding insects and the pathogen,
respectively. Roots emerging from seeds were evaluated for disease and then placed
with Tenebrio molitor larvae which were monitored for infection.
RESULTS: Plant disease symptoms were nearly absent for seeds treated with C. rosea, both
individually and in combination with Metarhizium spp. Furthermore, roots grown from seeds
treated with Metarhizium spp. caused significant levels of fungal infection in larvae when used
individually or combined with C. rosea. However, co-treated seeds showed reduced virulence
towards T. molitor as compared to treatments with Metarhizium spp. only.
CONCLUSIONS: This study clearly shows that seed treatments with both the entomopathogenic
fungus M. brunneum and the mycoparasitic fungus C. rosea can protect plant roots from insects and
disease. The dual-treatment approach to biological control presented here harmonizes well with the
ideals of IPM strategies.
66
1. INTRODUCTION
Crop production is consistently under pressure from various harmful organisms, including
plant pathogens and arthropod pests. Wheat is the most important cereal crop in the northern
hemisphere, Australia and New Zealand.1 Although current breeding and treatment programs have
greatly reduced the potential loss growers are in need of new and effective means for crop
protection.2 While use is continually increasing, in general, biological control agents (BCAs) of
pests and pathogens in agriculture have yet to become a mainstream option for crop producers.3
Many factors contribute to the reticence of the agricultural industry to turn full-heartedly to
biocontrol, including a lack of efficacy in consistent field performance and lack of economic
viability.3 An increased emphasis on fundamental research, especially in the areas of biology and
ecology of the beneficial organisms, has the potential to greatly improve biocontrol.3, 4
One
important question that needs to be addressed is whether BCAs of plant pests and pathogens can be
used simultaneously without mutually inhibiting the efficacy of the other BCA.5, 6
For biological control of arthropod pests members of the entomopathogenic fungal genus
Metarhizium (Metschnikoff) Sorokin (Hypocreales: Clavicipitaceae) are among the most promising
candidates.7 Metarhizium spp. have a worldwide distribution, a wide host range and have been
found to be effective against many important agricultural pests, including: grasshoppers, locusts,
mosquitoes, spittlebugs, thrips, white flies, and even ticks.7, 8
Furthermore, recent research has
highlighted their important role as root-colonizers with potential to aid in nutrient acquisition and
plant-growth promotion.9-11
For many important plant diseases Clonostachys rosea (Link:Fr.) Schroers, Samuels, Seifert
and Gams (syn. Gliocladium roseum Bainier) is a highly effective BCA; like Metarhizium, C.
rosea has a cosmopolitan distribution and is often naturally found in agricultural soil.12
C. rosea is
a broad-spectrum mycoparasite effective at reducing the growth and associated diseases of several
plant pathogenic fungi including: Alternaria spp., Bipolaris sorokiniana, Botrytis cinerea,
Fusarium culmorum, Sclerotinia sclerotiorum, and Verticillium dahlia.13-18
Several modes of
action towards other fungi have been attributed to C. rosea, including: nutrient competition,
mycoparasitism, induced resistance of the plant, and antimicrobial metabolite production and
detoxification of mycotoxins.12, 15, 19-21
Furthermore, many studies have prescribed strategies for
implementing C. rosea as a BCA.18, 22, 23
Clearly Metarhizium spp. and C. rosea have great
potential for use as BCAs in agriculture.
67
It is often necessary for agricultural producers to combat arthropod pest and plant pathogens
simultaneously. As Metarhizium spp. and C. rosea based products become more common it is
likely that they will be applied against different harmful organism (i.e., pests and diseases) on the
same crop; it is thus becoming increasingly important to understand how they might interact. As a
general mycoparasite C. rosea could potentially have deleterious effects on Metarhizium spp.
efficacy. In fact one study observed that M. anisopliae sensu lato was highly susceptible to several
mycoparasites including Clonostachys spp. in an in vitro host-range test.24
However, they also
found that co-application with M. anisopliae s.l. generally enhanced mycoparasite recovery from
the host insect and that virulence of the entomopathogenic fungi was not significantly altered.24
Additionally, C. rosea has been reported as an entomopathogenic fungus,25
and therefore may
contribute to biological control of arthropod pests. Also, at least one study reported that M.
robertsii has antifungal properties and was able to reduce Fusarium solani f. sp. phaseoli infections
in bean.26
Co-application of Metarhizium spp. and C. rosea could therefore have either
antagonistic, neutral or additive effects on their respective biological control efficiency;
undoubtedly investigations in to how these fungi interact when co-applied are highly important.
The aim of this study was to assess the effectiveness of two BCAs applied in combination as
seed treatments to control an insect pest and a plant pathogen. This was tested by treating
pathogen-infected seeds of two wheat varieties with a combination of C. rosea and Metarhizium
spp. (either M. brunneum or M. flavoviride). The seeds were grown under laboratory conditions
and the resulting plants were evaluated for disease development and then the roots were fed to
insect larvae which were monitored for mortality and fungal infection. Additionally, direct-
inoculations of insect larvae with the various individual and combined fungal treatments were
performed to evaluate the entomopathogenic potential by the fungi in isolation and together.
2. EXPERIMENTAL METHODS
2.1 Organisms
Five species of fungi were used in various experiments throughout this study. Three species
from the genus Metarhizium were included: M. brunneum (Mb) isolate KVL 04-57 which has the
same origin as the active ingredient of the commercial isolate Met52 (Novozymes, Salam,
Virginia);27
M. flavoviride (Mf) KVL 14-112, isolated in 2013 from Danish soil closely associated
with wheat roots using Tenebrio molitor L. (Coleoptera: Tenebrionidae) as bait insect; and M.
robertsii (Mr) KVL 12-35, isolated from Danish agricultural soil using T. molitor as a soil bait
insect.28
Additionally, one isolate of Clonostachys rosea (Cr) IK726 isolated from barley root,13
68
and one isolate of the wheat pathogen Fusarium culmorum (Fc) IK5 isolated from barley seed was
included.29
All fungal isolates are stored at -80 oC at the University of Copenhagen.
Two varieties of wheat (Triticum aestivum L.) were used in this study, ‘Jensen’ and
‘Nakskov’ supplied by Nordic Seed, Denmark. The seed lots were stored at -20 ºC. Before use
seeds were surface sterilized by soaking for 30 s in 70% ethanol and then 10 min in 4% sodium
hypochlorite (Sigma Chemical, MO, USA), followed by rinsing 3 times in ddH2O and air drying
overnight in a ventilation hood.
Insect infection assays were performed using T. molitor larvae (Avifauna, Copenhagen,
Denmark).
2.2 Fungal suspensions
Fungal suspensions were prepared for each of the five fungal species using fresh cultures of
each isolate which had been grown for 2-3 weeks on Potato Dextrose Agar (PDA) (Sigma
Chemical, MO, USA) at 24º C. Conidia were harvested with a sterile spatula and suspended in
0.05% Triton X-100 (Sigma Chemical, MO, USA), the suspension was then passed through cheese
cloth to remove hyphae, conidial clumps and loose agar. Each suspension was vortexed and
conidial concentrations estimated by counting in a haemocytometer (Fuchs-Rosenthal). Conidial
viability was determined by pipetting 20 µl of a diluted portion of the suspension onto agar medium
[4-ml SDA with 0.002% Benomyl active ingredient (Sigma-Aldrich, MO, USA)] and counting
conidia germination after 48 hours at 24ºC; all fungal isolates were observed to have greater than
95% viability.
2.3 Seedling disease and root-fed insect assay
A F. culmorum suspension of 1.5 × 105 conidia/ml was used to inoculate about 200 surface-
sterilized wheat seeds; the seeds were soaked for 30 min at 150 rpm in the F. culmorum suspension
(1:2 w/v). This was done for both ‘Jensen’ and ‘Nakskov’ varieties of wheat. Additionally, ~200
seeds of both varieties were soaked for 30 min in ddH20 as a non-infected control group. The seeds
were then removed from the suspension and allowed to air dry in a ventilation hood, after which
they were kept at 5 ºC and used within 10 days of preparation; this same batch of seeds was used for
both repetitions below.
The following 6 treatments of M. brunneum, M. flavoviride and C. rosea were prepared:
0.05% Triton X (control – no fungus), Mb, Mf, Cr, Mb+Cr, and Mf+Cr. Each fungal suspension
was prepared so that the final concentrations of Metarhizium spp. conidia were 1 × 108 conidia/ml
and the final concentration of C. rosea was 1 × 107 conidia/ml. These concentrations of
69
Metarhizium spp. and C. rosea were selected based on previous work showing effectiveness at
controlling their target insect or pathogen.13, 30
A surplus of both Fc infected and uninfected seeds
were soaked separately in each of the fungal suspension (or ddH2O for untreated control) for 5 min,
giving 12 separate treatments for each wheat variety. Twelve treated seeds were then evenly spaced
2 cm from the top edge of a 2-ply filter paper (58 × 29 cm) (Frisenette ApS, Denmark) which had
been moistened to saturation with ddH2O. The seeds were secured by placing a strip of filter paper
(7 × 58cm) along the top of the paper, which was rolled up in to a tube and placed standing upright
in a shallow reservoir of water, which was maintained throughout the experiment at approx. 5 cm in
depth. Each roll was wrapped in a piece of aluminum foil to keep seeds in the dark and reduce
evaporation and then placed under a growth lamp with 12/12 h light/dark regime at room
temperature (21±2 ºC) for 14 days. For each treatment combination (Fc/No-Fc, Mb/Cr, Mf/Cr
combinations, and wheat varieties), two pseudo-replicate paper rolls were prepared resulting in 48
paper rolls prepared for each experimental repetition. Additionally, 5-6 seeds from each treatment
were placed on PDAY media to check for seed viability and the presence of the applied fungus
(Supplemental Figure 1).
On day 13 each paper roll was unrolled and plants were assessed for disease severity using
an index from 0 to 4 as previously suggested,13
viz.: 0=healthy plant, 1= slightly brown
coleoptile/roots, 2=moderately brown coleoptile and/or roots, 3=severe browning of the coleoptile
and/or roots, 4=dead plant (Supplemental Figure 2). All disease assessments were done by the
same person to avoid subjective inconsistencies; also the treatments were assessed randomly and
blindly to avoid any treatment expectations. After the assessment the paper rolls were re-rolled and
incubated for one additional day. This entire procedure was repeated twice at different times with
new plants and fungal suspensions.
Insect assay were performed using the methods described by Keyser et al.30
In short, petri
plates (60×15 with vents, Greenbio One, Hungary) were lined with a single sheet filter paper (Size
55, VWR international, France) and moistened with 200 µl of ddH20; for each treatment 3 replicate
plates were prepared. The top 10 cm, starting just below the seed, for all of the roots from a single
treatment (both pseudo-replicate rolls) were combined, cut into 1-2 cm pieces, mixed together, and
0.2-0.3 g of root material was added to each of the three replicate petri plate per treatment. After
adding the cut-root sections, ten T. molitor larvae were added to each plate. Each treatment set of 3
petri plates were stacked with a forth empty plate below, rubber banded together and placed upright
in a plastic container containing moist paper towels for humidity. Mortality was assessed daily and
70
the order of the petri plates in each stack was cycled each day with the empty plate always on the
bottom. Dead insects were removed and placed in medicine cups with moist filter paper to observe
for mycosis. The dual concept of the experimental design is outlined in Supplemental Figure 3.
2.2 Insect infection bioassay
Two separate infection bioassay experiments were performed: a low dose (1 × 105
conidia/ml) and a high dose (1 × 107 conidia/ml). For each experiment the following 16 treatments
were prepared: 0.05% Triton X (control), Mb, Mf, Mr, Cr, Mb+Cr, Mf+Cr, Mr+Cr, Fc, Mb+Fc,
Mf+Fc, Mr+Fc, Cr+Fc, Mb+Cr+Fc, Mf+Cr+Fc, and Mr+Cr+Fc. For each bioassay the fungal
treatments were prepared so that each fungal species included in the particular treatment had the
same number of conidia per ml; e.g., in the low dose treatment Mb+Cr had 1 × 105 conidia/ml of M.
brunneum and 1 × 105 conidia/ml of C. rosea. Suspensions were kept at 5 ºC until use which was
always within 24 h of preparation.
Thirty T. molitor larvae were prepared in three petri plates as in the root-insect assay above.
In each petri plate the 10 larvae were individually inoculated by pipetting 5 µl of a designated
suspension. Mortality was assessed daily and the order of the petri plates in each stack was cycled
each day. Dead insects were removed and placed in medicine cups with moist filter paper in order
to observe mycosis. This entire procedure was repeated two or three times for the 1 × 105
conidia/ml and for the 1 × 107 conidia/ml doses, respectively.
2.4 Statistics
For the root assay data and the infection bioassay data the virulence of the treatment groups
to T. molitor was estimated using a survival analysis.31
A comparison of the survival curves was
performed for biologically distinct groups of treatments. For the infection bioassay each conidial-
concentration bioassay was analyzed separately, for each concentration there were four distinct
groups, including, 1 (no Metarhizium): Untreated control, Cr, Fc, and Cr+FC; 2 (M. brunneum):
Mb, Mb+Cr, Mb+Fc, and Mb+Cr+Fc; 3 (M. flavoviride): Mf, Mf+Cr, Mf+Fc, and Mf+Cr+Fc; and 4
(M. robertsii): Mr, Mr+Cr, Mr+Fc, and Mr+Cr+Fc. For the root assay three groups were evaluated
separately, these were the same as the above groups 1, 2 and 3. The following procedures were
used to analyze each of the groups: first, a cox proportional hazard (PH) model was performed on
the survival curves; next, a chi-square test of the PH model was used to determine if there was
significant variation between the treatments within the model; lastly, if the chi-squared test yielded
a p-value less than 0.05 a pairwise comparisons was done using a cox mixed model with trial as the
random factor, and the p-values were adjusted using the Bonferroni method.
71
The data from the disease index was viewed as categorical; therefore each seed represented
an individual data point and was not averaged with other seed of the same treatment. To simplify
the analysis of the disease severity data was divided into two classes, plants receiving an index
value of 0 or 1 and plants designated as 2 or greater on the disease index scale. A chi-squared test
for independence was performed to determine whether there were differences in among the 12
fungal-treatment combinations. Further analyzes were then performed on two specific treatment
groups; viz. group 1: untreated, Mb, Mf, Cr, Mb + Cr, Mf + Cr, Cr + Fc, Mb + Cr + Fc, and Mf + Cr
+ Fc; and group 2: Fc, Mb + Fc, and Mf + Fc. This additional analysis was done using a
generalized linear mixed model (glmer) in R.
Fungal mycosis on dead larvae between treatments was evaluated using a generalized linear
model for binomial data. The proportions of dead insects with mycosis to dead insect with no
mycosis between treatments were compared. All of the analyses were performed in RStudio
(version 0.97.551).
3. RESULTS
3.1 Root-insect assay
When comparing the survival curves for ‘Jensen’ and ‘Nakskov’ wheat varieties separately,
Cr and Fc treatments which did not include Metarhizium spp. were not significantly different from
each other and the untreated control (2 = 6.9, df = 3, p = 0.07; and
2 = 0.45, df = 3, p = 0.9,
respectively) (Figs. 1a and 1b). In contrast, there was a significant effect of treatment for ‘Jensen’
and ‘Nakskov’ when comparisons included the untreated control and Cr and Fc treatments
combined with M. brunneum (2 = 133.6, df = 4, p < 0.0001; and
2 = 144.5, df = 4, p < 0.0001,
respectively); for both varieties the untreated control had significantly more survival (>95%) than
the other treatments. For both varieties the highest virulence was observed when the seeds were
treated with M. brunneum alone (Figs. 1c and 1d).
A significant effect of treatment was observed for both ‘Jensen’ and ‘Nakskov’ wheat in
comparisons which included the untreated control and Cr and Fc in combination with M.
flavoviride (2 = 49.6, df = 4, p < 0.0001; and
2 = 38.5, df = 4, p < 0.0001, respectively).
However, the treatments including F. culmorum did not reduce survival in comparison to the
untreated control of ‘Jensen’ (Fig. 1e) while all treatments that included M. flavoviride differed
from the control for the ‘Nakskov’ variety (Fig. 1f).
An analysis of the proportion of dead insects with observed mycosis to the total number of
dead insects in ‘Jensen’ indicated that there was an effect of treatment when either M. brunneum (2
72
= 9.6, df = 3, p = 0.02) or M. flavoviride (2 = 54.6, df = 3, p = 0.006) were included in the
treatments. However, an adjusted pairwise comparison of the treatments that included M.
brunneum was unable to identify significant differences among the treatments (Fig. 2a). For M.
flavoviride a significantly greater proportion of dead insects with observed mycosis were detected
when exposed to M. flavoviride alone than for the combined Mf+Cr treatment (Fig. 2b).
Mycosis on dead insects exposed to the roots of ‘Nakskov’ had a significant effect of fungal
treatment when M. brunneum (2 = 10.4, df = 3, p = 0.01) and M. flavoviride (
2 = 10.9, df = 3, p =
0.01) were included. A pairwise comparison revealed that for the M. brunneum treatments a
significantly greater proportion of dead insects had mycosis when treated with M. brunneum alone
than in the combination Mb+Cr (Fig. 2c). When the treatment included M. flavoviride only, a
significantly greater proportion of dead insects had mycosis than when combined with F. culmorum
(Fig. 2d).
3.2 Root disease
There was a significant effect of treatment on the root disease severity (2 = 679.8, df=11,
p<0.0001, Fig. 3). However, a subsequent analysis revealed that there were no differences between
the three treatments that included F. culmorum but did not include C. rosea (i.e., Fc, Mb + Fc, and
Mf + Fc) (2 = 184.3, df=2, p=0.85). Furthermore, the six treatments without F. culmorum and the
three treatments including both F. culmorum and C. rosea did not differ significantly (i.e., Mb, Mf,
Cr, Mb+Cr, Mf+Cr, Cr+Fc, Mb+Cr+Fc, and Mf+Cr+Fc) (2 = 59.6, df=8, p=0.26).
3.3 Infection bioassay of directly inoculated larvae
3.3.1 Low dose: No effects on T. molitor survival of Cr and Fc treatments were observed
when Metarhizium spp. were not included (2 = 2.2, df = 3, p = 0.52) (Fig. 4a). An analysis
evaluating the untreated controls with the treatments that included M. brunneum, M. flavoviride or
M. robertsii showed a significant decrease in survival for all three Metarhizium species (2 = 179.1,
df = 4, p < 0.0001; 2 = 48, df = 4, p < 0.0001;
2 = 145.1, df = 4, p < 0.0001, respectively) (Figs.
4c, 4e, and 4g). An analysis of the treatment combinations that included either of the Metarhizium
spp. isolates (excluding the untreated control) revealed no significant effect of treatments that
included M. brunneum (2 = 0.34, df = 3, p = 0.95) (Fig. 4c) as well as the treatments that included
M. flavoviride (2 = 5.81, df = 3, p = 0.12) (Fig. 4e). However, a significant effect was observed for
the treatments which included M. robertsii (2 = 9.1, df = 3, p = 0.02) where M. robertsii in
combination with F. culmorum had reduced virulence as compared to M. robertsii when used alone
(Fig. 4g).
73
3.3.2 High dose: An effect of treatment on T. molitor survival was observed when
Metarhizium spp. isolates were not included (2 = 13.8, df = 3, p = 0.003), and pairwise
comparisons revealed that the untreated control was significantly different from the Cr+Fc
treatment (z = 2.9, p = 0.017); after 14 days the average mortality of the Cr+Fc treatment was
18.9% whereas the average mortality of the control group was 3.3% (Fig. 4b). An effect of
treatment was observed in all groups in an analysis evaluating the untreated controls and treatments
including either M. brunneum, M. flavoviride, or M. robertsii (2 = 253.3, df=4, p < 0.0001;
2 =
187.6, df = 4, p < 0.0001; 2 = 277.9, df = 4, p < 0.0001, respectively). Pairwise comparisons
among these treatments revealed that the untreated control differed significantly from all treatments
that contained either Metarhizium species (Figs. 4d, 4f, and 4h). An additional analysis was
performed comparing the treatment combinations with each Metarhizium spp. isolate but excluding
the untreated control group. No significant difference was observed for those with M. brunneum or
M. robertsii (2 = 1.1, df = 3, p = 0.77;
2 = 0.7, df = 3, p = 0.86, respectively). However, an effect
of treatment was observed for those with M. flavoviride (2 = 14.3, df = 3, p = 0.002); in a pairwise
comparison of the treatments M. flavoviride alone was more virulent than when F. culmorum was
included in the treatments (z = 3.8, p = 0.0007; and z = 4.1, p = 0.0002, respectively) (see fig. 4f).
3.3.3 Mycosis: No significant effect of treatment on the proportion of dead insects with
mycosis to all dead insects was observed for M. brunneum or M. robertsii treatments at the low
dose (2 = 2.14, df = 3, p = 0.54;
2 = 7.53, df = 3, p = 0.056, respectively (Figs. 5a and 5c). At the
low dose for the M. flavoviride treatments a significant effect for treatment was observed (2 = 7.97,
df = 3, p = 0.046), however a pairwise comparison with adjusted p-values failed to identify the
differences (Fig. 5b). For the high dose when the treatments that included M. brunneum were
compared to each other a difference in the proportions for the overall model was observed (2 =
49.9, df = 3, p = 0.03), however a pairwise comparison with adjusted p-values failed to identify the
differences (Fig. 5d). There was an effect of treatment for the proportion of dead insects with
mycosis for those treated with M. flavoviride (2 = 90, df = 3, p < 0.0001), with the M. flavoviride
only treatment showing higher proportion of mycosis than when combined with other fungi (Fig.
5e). No significant effect of treatment on the proportion of dead insects with mycosis to dead
insects was observed for the treatments with M. robertsii (2 = 4.36, df = 3, p = 0.224) (Fig. 5f).
4. DISCUSSION
An integrated biological control treatment of the entomopathogenic fungi M. brunneum or
M. flavoviride combined with the mycoparasite C. rosea on wheat seeds resulted in almost complete
74
reduction of F. culmorum plant infections; and, in the case of the M. brunneum/C. rosea treatment,
insect mortality after exposure to wheat roots as high as 80%. These data clearly show that
cooperative biological control of two very different harmful organisms can be achieved utilizing the
combination of M. brunneum and C. rosea as wheat seed treatment. Others studies have also shown
that mixtures of BCAs can be effectively used against pests and pathogens,24, 32, 33
but this is the
first to focus on a seed borne pathogen and insects feeding on roots.
Survival of insects exposed to roots from treatments of M. brunneum combined with other
fungi was greater than those in the M. brunneum only treatment. However, when the same fungi
were exposed directly to the insects the virulence of M. brunneum was not affected by combination
with other fungi. These results could suggest that the reduced virulence seen in the plant assay was
either due to an indirect interaction (e.g., competition for resources) or a direct antagonism by the
other fungi as consequence of lower acquired dose of M. brunneum by the insects in the plant assay
allowing for the manifestation of subtle effects. The first hypothesis is supported by the observation
that the reduced virulence was seen in all combinations not just those with C. rosea, indicating that
the response is not specifically associated with the mycoparasitic ability of C. rosea. Krauss et. al
found that two isolates of M. anisopliae s.l. were susceptible to C. rosea mycoparasitism,24
however
this was tested in vitro by observing whether C. rosea was able to grow on agar media already
colonized by M. anisopliae s.l. While this method does indicate mycoparasitism against M.
anisopliae s.l., it is unlikely to effectively predict how the two fungi will interact when neither is yet
established and/or under more natural conditions. In fact in crop production systems there will be a
strong competition from the native soil microbiota. As in the current study, Krauss et al. observed
that co-inoculation of the two fungi did not reduce Metarhizium spp. virulence to insects.24
In the plant-insect assay with M. flavoviride some of the combined fungal treatments had
greater survival than the M. flavoviride only treatment; in fact on the wheat variety ‘Jensen’,
combinations of M. flavoviride with F. culmorum and these two fungal species combined with C.
rosea did not differ significantly from the untreated controls. We also observed comparable trends
for the same fungal treatments in the direct insect inoculation assay at the high dose. The isolate of
M. flavoviride used in this study was selected because it was observed to form inhibition halos
when grown on agar media with F. culmorum (C.A. Keyser, pers. obs.), indicating that there might
be some antifungal compounds produced by one or both of the species which could account for the
reduced virulence observed in the combined treatments. However, there was still a relatively high
level of infection of the directly-inoculated insects in the Mf+Cr, Mf+Fc and Mf+Fc+Cr high-dose
75
treatments suggesting that any direct interaction between the fungal isolates was likely minimal.
The particular isolate of M. flavoviride was previously found to be less virulent than the isolate of
M. brunneum against T. molitor larvae;30
a relatively low dose resulting in limited infection in the
host mortality is likely to be sensitive to effects of other fungi which might account for the reduced
virulence in the combination treatments.
Isolates of C. rosea and Fusarium spp. have been observed to infect insects,25, 34
however in
this study there was no indication that any of the C. rosea or F. culmorum isolates used were
pathogenic towards T. molitor. Although the direct inoculation assay at the high dose showed that
insects exposed to C. rosea and F. culmorum had significantly lower survival than the untreated
control, no fungal mycosis from the dead insects was detected suggesting that the slightly lower
survival was not due to fungal pathogenicity as defined by Koch’s postulates.35
Furthermore, this
observation could not be ascribed to inability of the two fungi to colonize wheat roots since dilution
plating on semi-selective media of root subsamples from the feeding experiments confirmed that
both fungi were present on roots grown from seed treated with the respective fungi (data not
shown). In a study with leaf-cutting ants it was shown that a combination of a virulent isolate of M.
anisopliae s.l. with an avirulent isolate of Aspergillus flavus resulted in the same level of virulence
as a M. anisopliae s.l. only treatment despite the combined treatment having only half as many M.
anisopliae s.l. conidia as the latter.36
They also observed that in the combined treatment more dead
insects showed mycosis by A. flavus than M. anisopliae s.l. and concluded that the avirulent A.
flavus, once inside the host, was able to out-compete the M. anisopliae s.l. isolate when the host
immune responses were compromised.36
In the present study, both C. rosea and F. culmorum
isolates grow more rapidly on artificial media than Metarhizium spp. isolates at equal conditions
(C.A. Keyser, pers. obs.); however, no C. rosea or F. culmorum mycosis was observed in any
insects, suggesting that the same mechanism of co-infection observed by Hughes and Boomsma is
not applicable to our fungal combinations.36
It could be speculated that the two fungal isolates
produce metabolites being toxic to the larvae.
The isolate of C. rosea was a highly effective BCA of F. culmorum in the current study,
corroborating results of other studies using the same isolate.37
Combination with either of the
Metarhizium spp. isolates did not affect the efficacy of C. rosea in reducing F. culmorum disease
manifestations. However, since the dose of C. rosea used in this study was sufficient to almost
completely control the plant pathogen any potential additive effects derived from Metarhizium spp.
would likely not be observed. Furthermore, additive effects would be unlikely to expect using the
76
current Metarhizium spp. isolates, since neither of the isolates tested in the plant assay were
observed to have an effect against F. culmorum alone. Antagonism against F. solani in bean plants
by an isolate of M. robertsii has been reported.26
In that study a significant reduction in F. solani
infection on bean roots was observed when sterile soil was pre-inoculated with F. solani and M.
robertsii compared to F. solani only treatments. This study also reported reduced germination of F.
solani conidia when grown in M. robertsii cell-free culture media; from this they concluded that the
actively growing M. robertsii isolate produced compounds that inhibited F. solani growth.26
While
no indication of Metarhizium spp.-mediated antagonism against F. culmorum was observed in the
current study, several important differences exist between the two studies which could have
accounted for the different results, including: species of Metarhizium and Fusarium used,
experimental plant species, inoculation method, and the fact that Sasan and Bidochka allowed an
establishment period for M. robertsii and F. solani in the soil before introducing the bean seeds.26
Biological control of plant pests and pathogens has enormous potential to improve
sustainable agricultural production and harmonizes with the ideals of IPM strategy. Nevertheless,
in order for BCAs to be used effectively and consistently we must improve our basic understanding
of how they interact in the field - especially how they work when applied in combination. While
further studies in soil microcosms and under field conditions are necessary, the current study clearly
demonstrated that entomopathogenic fungi from the genus Metarhizium and the plant pathogen
mycoparasite C. rosea can potentially be used in concert to control both belowground insects and
seed borne pathogens in a single treatment.
5. ACKNOWLEDGEMENTS
We would like to give special thanks to Line Lykke, Lærke Thordsen, Martina Falagiarda,
Louise Lee Munk Larsen for their technical assistants in this study. We would also like to give
thanks to Dr. Bernhardt M. Steinwender for his theoretical input and contribution into the
experimental design. This research was funded by a PhD grant to C.A.K from the Plant Biosystems
Elite Environment at the University of Copenhagen.
77
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79
Table
Table 1. Treatment combination with respective abbreviation and experiments in which they were
included.
Abbreviation Treatment See
d t
rea
tmen
t/
roo
t ass
ay
Dir
ect
ino
cula
tio
n
1 ×
10
5
Dir
ect
ino
cula
tio
n
1 ×
10
7
Untreated Treated with ddH2O as a control x x x
Cr Clonostachys rosea x x x
Fc Fusarium culmorum x x x
Cr + Fc Clonostachys rosea + Fusarium culmorum x x x
Mb Metarhizium brunneum x x x
Mb + Cr Metarhizium brunneum + Clonostachys rosea x x x
Mb + Fc Metarhizium brunneum + Fusarium culmorum x x x
Mb + Cr + Fc Metarhizium brunneum + Clonostachys rosea + Fusarium culmorum x x x
Mf Metarhizium flavoviride x x x
Mf + Cr Metarhizium flavoviride + Clonostachys rosea x x x
Mf + Fc Metarhizium flavoviride + Fusarium culmorum x x x
Mf + Cr + Fc Metarhizium flavoviride + Clonostachys rosea + Fusarium culmorum x x x
Mr Metarhizium robertsii x x
Mr + Cr Metarhizium robertsii + Clonostachys rosea x x
Mr + Fc Metarhizium robertsii + Fusarium culmorum x x
Mr + Cr + Fc Metarhizium robertsii + Clonostachys rosea + Fusarium culmorum x x
80
Figure Legends
Figure 1. Mean daily survival (%) of T. molitor larvae over a 14 day period after exposure to wheat
roots. Roots were grown for two weeks from seeds of two wheat varieties that had been exposed
separately to one of 12 various treatments which included untreated seeds and all combinations of
Metarhizium sp., Clonostachys rosea (Cr) and Fusarium culmorum (Fc). Survivorship curves
represent each wheat variety having received treatments without Metarhizium spp. (a, b), with M.
brunneum (c, d) or M. flavoviride (e, f). Within each graph the legend box contains a figure key
designating treatments and significance levels. Treatments with different letters are significantly
different while “ns” indicates no significant differences among treatments.
Figure 2. Total larval mortality of T. molitor and proportion of Metarhizium spp. mycosis observed
on dead larvae (black) after exposure to wheat roots for 14 days. Dead insects without mycosis are
represented by grey bar for all treatments. Mycosis was only observed on insects exposed to roots
treated with either M. brunneum (a, c) or M. flavoviride (b, d) (n=90 exposed larvae per treatment)
with the two varieties of wheat tested separately. Within each graph, statistical analyses of data
apply only to the proportion of dead larvae with mycosis. Lower case letters above the bars
represent significance levels in relation to the other treatments.
Figure 3. Proportions of wheat plants in each disease-severity rank grouped by treatment across
both experimental repetitions assessed after 13 days. Data from both wheat varieties of wheat were
combined. Only germinating seeds were assessed for disease thus number of observations varied
among treatments.
Figure 4. Mean daily survival (%) of T. molitor larvae over a 14 day period after treatment. Larvae
were directly inoculated with 5 µl of a designated fungal suspension of either ‘low’ (a, c, e, g) or
‘high’ dose (b, d, f, h) which included control inoculation and all combinations of Metarhizium sp.,
Clonostachys rosea (Cr) and Fusarium culmorum (Fc). Each individual graph contains a figure
key which designates the treatment; within each graph significantly different treatments are
presented by different letters while “ns” indicates no significant effect of treatment.
Figure 5. Total larval mortality of T. molitor and proportion of mycosis of Metarhizium spp.
observed on dead larvae (black) after direct inoculation with a fungal treatment or untreated control.
Dead insects without mycosis are represented by grey bars for all the treatments. Mycosis was only
observed on insects treated with either M. brunneum (a, d), M. flavoviride (b, e) or M. robertsii (c,
f) (n=90 exposed larvae per treatment); for the high dose experiment mycosis on dead insects was
only checked for two of the three repetitions, for the low dose mycosis was checked on both
repetitions. Lower case letters above the bars represent significance levels in relation to the other
treatments within the same graph.
81
Figure 1
20
40
60
80
100
20
40
60
80
100
Su
rv
iva
l o
f T
. m
oli
tor
larv
ae (
%)
Wheat variety Jensen Wheat variety Nakskov
b
e f
dc
a
nsnsns
CrFcCr+Fc
ns Untreated
nsnsns
CrFcCr+Fc
ns Untreated
bbaa
Mf
Mf+CrMf+FcMf+Cr+Fc
a Untreatedcbcbbc
Mf
Mf+CrMf+FcMf+Cr+Fc
a Untreated
cbbb
Mb
Mb+CrMb+FcMb+Cr+Fc
a Untreatedcbbb
Mb
Mb+CrMb+FcMb+Cr+Fc
a Untreated
2 4 6 8 10 12
0
20
40
60
80
100
Time (d)
2 4 6 8 10 12 14
82
Figure 2
83
Figure 3
Treatment
Pla
nts
wit
hin
ea
ch
dis
ease
-sev
erit
y c
lass
(%
)
0
20
40
60
80
100
Healthy Plant
Slightly brown
Moderately brown
Severe browning
Dead
Un
trea
ted
Mb
Mf
Cr
Mb
+ C
r
Mf
+ C
r
Fc
Mb
+ F
c
Mf
+ F
c
Cr
+ F
c
Mb
+ C
r +
Fc
Mf
+ C
r +
Fc
84
Figure 4
Time (d)
2 4 6 8 10 12
0
20
40
60
80
100
Su
rviv
al
of
T.
moli
tor
larvae (
%)
1 x 105 conidia/ml 1 x 107 conidia/ml
20
40
60
80
100
20
40
60
80
100
20
40
60
80
100
2 4 6 8 10 12 14
b
e f
dc
a
g h
cbcbb
Mf
Mf+CrMf+FcMf+Cr+Fc
a Untreatedbbbb
Mf
Mf+CrMf+FcMf+Cr+Fc
a Untreated
bbbb
Mb
Mb+CrMb+FcMb+Cr+Fc
a Untreated
nsnsns
CrFcCr+Fc
ns Untreated
dcdbcb
Mr
Mr+CrMr+FcMr+Cr+Fc
a UntreatedMr
Mr+CrMr+FcMr+Cr+Fc
Untreatedbbbb
a
ababb
CrFcCr+Fc
a Untreated
bbbb
Mb
Mb+CrMb+FcMb+Cr+Fc
a Untreated
85
Figure 5
86
Supplemental Figures
Supplemental figure 1: Treated wheat seeds were placed on PDAY media to assess viability of the
seeds and fungal treatments. Pictures of ‘Nakskov’ (top) and ‘Jensen’ (bottom) wheat varieties
after 3 (left) and 10 (right) days.
Supplemental figure 2: Disease index used to asses severity of F. culmorum infection in wheat
plants after 13 days growth in filter paper rolls with 12/12 h light/dark.
Supplemental figure 3: An illustration describing the experimental design of the wheat-seed
treatment and root-insect infection assay.
87
Supplemental figure 1
C. ro
sea
F. cu
lmoru
m
C. ro
sea a
nd
F. cu
lmoru
m
M. brunneum M. flavoviride M. brunneum M. flavoviride C
. ro
sea
F. cu
lmoru
m
C. ro
sea a
nd
F. cu
lmoru
m
88
Supplemental figure 2
0 =
Healthy
plant
1 =
Slightly
brown
coleoptile/
roots
2 =
Moderately
brown
coleoptile
and roots
3 =
Severe
browning
of
coleoptile
and roots
4 =
Dead plant
89
Supplemental figure 3
Symptoms of
Fusar ium
infection
1. Fusarium infected
and control seeds are
treated with biocontrol
agents
2. Seeds are allowed
germinate and grow for
14 days
3. Plants are assessed
for disease and roots
are fed to insect larvae
90
Manuscript 3
DIVERSITY OF METARHIZIUM FLAVOVIRIDE POPULATIONS ASSOCIATED WITH ROOTS OF CROPS IN
DENMARK
Chad A. Keyser, Henrik H. de Fine Licht, Bernhardt M. Steinwender & Nicolai V. Meyling
Status: Manuscript
91
Diversity of Metarhizium flavoviride populations associated with roots of crops in Denmark
Chad A. Keyser*, Henrik H. de Fine Licht, Bernhardt M. Steinwender, and Nicolai V. Meyling
Department of Plant and Environmental Sciences, University of Copenhagen, Thorvaldsensvej 40,
1871 Frederiksberg, Denmark
*Corresponding author: Chad A. Keyser, Department of Plant and Environmental Sciences,
University of Copenhagen, Thorvaldsensvej 40, stair 2, 3rd floor, B321,
1871 Frederiksberg, Denmark
Email: [email protected]
Keywords
AFLP, Entomopathogenic fungi, soil baiting, rhizosphere association, endophyte
92
Abstract
Ecological studies assessing the natural occurrence and community structure of
entomopathogenic fungi are important to understanding their role in insect host regulation;
however, there has been an acute lack of studies on the distribution of fungi in the genus
Metarhizium. The objective of the present research was to evaluate the occurrence, diversity and
community structure of Metarhizium spp. isolates obtained from roots and root-associated soil of
wheat, oilseed rape, and bordering uncultivated grazed pastures at three geographically separated
agricultural fields in Denmark. Of the132 Metarhizium isolates obtained, morphological data and
sequencing of the rDNA intergenic spacer region (IGS) revealed that 118 belonged to Metarhizium
flavoviride, 13 to M. brunneum and one M. majus. Further characterization of intraspecific
variability within M. flavoviride by unspecific markers (amplified fragment length polymorism,
AFLP) was used to evaluate diversity and potential crop and/or area associations. A high level of
diversity among the M. flavoviride isolates was observed, indicating that the isolates were not of the
same clonal origin. However, due to insufficient loci in the AFLP analysis we were not able to
determine significant haplotype groupings or confirm any habitat associations of these isolates. We
suggest that the development of more specific molecular markers would greatly improve the ability
to evaluate M. flavoviride diversity which has largely been ignored. This study represents the first
in-depth analysis of the molecular diversity within a large isolate collection of the species M.
flavoviride.
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1. Introduction
The predominantly entomopathogenic fungal genus Metarhizium (Hypocreales:
Clavicipitaceae) has a global distribution (Kepler et al., 2014; Roberts and St. Leger, 2004;
Zimmermann, 2007) and several species have been intensely researched for their pest control
potential. Discordantly, limited focus has been given to the assessment of natural occurrence and
distribution of this widespread fungal genus. Knowledge of the compositions of entomopathogenic
fungal communities and structure of their populations is important to understand their contribution
to host regulation and potential for conservation biological control (Meyling and Eilenberg, 2007).
Evaluation of fungal diversity and community structure depends heavily on criteria for
species identification. With few morphological distinct features, species referred to as M. anisopliae
in the literature could belong to several different species if no explicit molecularly based
identification has been conducted. Bischoff et al. (2009) revised the taxonomy of the M. anisopliae
lineage based on a multigene phylogeny and resolved nine species within what could
morphologically be considered as M. anisopliae sensu lato. Recently, the taxonomy of the whole
genus Metarhizium was revised leading to the inclusion of other genera as well as elevation of some
of the former M. flavovoride variants to species level (Kepler et al., 2014). Kepler and Rehner
(2013) further specified additional genomic regions for species identification. Molecularly based
evaluation of the diversity of Metarhizium communities should therefore be included in studies of
natural occurrence and distribution to provide full recognition of diversity.
In temperate climatic regions, Metarhizium spp. are predominantly isolated from the soil
environment (Vega et al., 2012). Surveys of entomopathogenic fungi from soil samples conducted
at different geographical locations have shown that M. anisopliae s.l. can be abundantly isolated
from managed ecosystems (e.g. Bidochka et al., 1998; Goble et al., 2010; Inglis et al., 2008;
Klingen et al., 2002; Meyling et al., 2011; Steinwender et al., 2014; Sun et al., 2008). However,
few studies have evaluated Metarhizium community structure using explicit molecular
characterization. In Denmark, Meyling et al. (2011) isolated M. anisopliae s.l. from an agricultural
field and Steinwender et al. (2014) subsequently showed that the Metarhizium community was
composed of several species, predominated by M. brunneum. Further characterization with
microsatellite markers revealed several co-occurring multilocus genotypes within both M.
brunneum and M. robertsii (Steinwender et al., 2014).
Naturally occurring Metarhizium spp. were recently isolated from roots of different plants
(Fisher et al., 2011; Wyrebek et al., 2011). Some level of plant association was indicated by a
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predominance of M. robertsii found on roots of grasses as compared to M. brunneum which was
mostly recovered from roots of woody plants (Wyrebek et al. 2011). Sampling roots of different
plants from an ecosystem might therefore reveal the Metarhizium diversity of an area since similar
M. brunneum and M. robertsii multilocus genotypes can be repeatedly isolated from roots and soil
samples at the same site (Steinwender, 2013). However, the entomopathogenic fungal community
structure of the soil can differ markedly between agricultural fields within relatively close
proximity. Although Meyling et al. (2011) mostly isolated M. anisopliae s.l. (predominantly M.
brunneum) another agricultural field in Denmark showed low occurrence of M. anisopliae s.l.
(Meyling and Eilenberg, 2006). At the latter site, M. flavoviride was isolated more frequently than
M. anisopliae s.l. indicating location specific fungal communities.
The aim of the current study was to evaluate the occurrence, diversity and community
structure of Metarhizium spp. isolates obtained from roots and root associated soil of different
common crops at geographically separated agricultural fields in Denmark. Using such a sampling
scheme we expected to reveal potential crop and/or location association. Based on recent evidence
(Steinwender et al., 2014) we expected to isolate M. brunneum most frequently, however the study
resulted in a predominance of M. flavoviride isolates. Since the available microsatellite markers
developed for M. anisopliae s.l. are not specific for M. flavoviride (Steinwender, 2013) we chose to
characterize the intraspecific variability within M. flavoviride by unspecific markers to evaluate
diversity and potential crop and/or area associations.
2. Material and Methods
2.1 Field sampling
Three geographically separated areas were located in Sjælland, Denmark, including: Fårevejle
(55.78º N, 11.43 ºE), Skibby (55.75 º N, 11.99 ºE), and Taastrup (55.67 º N, 12.3 ºE). Within each
sampling site three agricultural fields were identified resulting in a 2-level nested design. The fields
included one field of winter wheat (Triticum aestivum), one with oilseed rape (Brassica napus), and
a permanent grass field that had been without cultivation for more than 20 years.
From each of the nine fields, 50 root samples were collected by walking from one edge, a
transect of the field towards the center; a plant/soil sample was collected every 3-4 meters using a
long-handled weeding fork. Each sample was placed individually in a pre-labeled 10 liter plastic
bag along with about 500 g of root-associated soil adhering to the root system. The three fields
from each geographic area were sampled on the same day; collections were made on three
95
consecutive days from July 23 – July 25, 2013. After collection samples were placed at 5 ºC until
they were processed within 30 days.
2.2 Fungal isolation
2.2.1 Selective media: From each sample a section of the root was removed and washed with
ddH2O to remove loose soil. A portion (~0.5 ± 0.25 g) of the washed root was then cut in to small
pieces (~2 mm) and placed in 10 ml ddH2O and homogenized using a rotary homogenizer
(Wyrebek et al., 2011). 200 µl of homogenate was then spread onto a selective agar media adapted
from Fernandes et al. (2010b), which consisted of: 39 g potato dextrose agar (Sigma Chemical, MO,
USA), 1g yeast extract (Merck KgaA, Darmstadt Germany), 0.25 g cyclohexamide (Sigma
Chemical, MO, USA), 0.5 g chloramphenicol (Sigma Chemical, MO, USA), 0.02 g dodine
(Agriphar, Belgium) (all weights per liter); two plates for each root sample were prepared. After
inoculation the plates were incubated for 28 days at 22 ºC in darkness and checked on day 7, 14, 21
and 28. Colonies morphologically identified as Metarhizium were transferred to a clean plate of
potato dextrose agar supplemented with 1% yeast extract (PDAY) using a sterile inoculating needle
to obtain pure cultures.
2.2.2 Soil baiting: The soil baiting method used in this study was adapted from Zimmermann
(1986). The soil from each sampling site was allowed to air dry over night at room temperature and
then re-moistened with ddH2O so that it was “slightly damp”. Soil (~120 ml) was then placed in a
plastic cup (155 ml) leaving 1 cm of airspace at the top. Prior to filling the cup large debris and
clumps were removed or broken up. Ten healthy 4-5th
instar Tenebrio molitor L. (Coleoptera:
Tenebrionidae) larvae were then added to each cup. A lid with ventilation holes was placed on top
of each sample and the cups were stacked upside down – so that the larvae were beneath the soil –
in a box. Every 1-2 days the box was rotated so that the orientation of the cups shifted, forcing the
T. molitor larvae to move through the soil substrate increasing the likelihood they would come in
contact with pathogenic microorganism in the soil. Insect survival was checked weekly; dead
insects were removed, washed with ddH2O and placed in a medicine cup with a moist piece of filter
paper to check for mycosis. Using a sterile inoculation needle, fungal isolations were made from
insect cadavers with mycosis and plated on PDAY media. After 14 days growth colonies were
evaluated, morphologically identified and Metarhizium spp. isolates were kept for further studies.
The number of isolate from each location and field type were assessed with a one-way
analysis of variance using the analysis of variance (AOV) command in R. All of the analyses were
performed in RStudio (version 0.97.551).
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2.3 PCR amplification and sequencing
For each Metarhizium isolate, lyophilized mycelium was prepared by growing cultured
isolates in liquid media (Steinwender et al., 2014) for four days at 22 ºC on a stirring table at 170
rpm. Mycelium was separated using a vacuum filtration system, frozen over night at -20 ºC and
lyophilized. DNA was extracted from the lyophilized mycelia using the DNeasy Plant Mini Kit
(QIAGEN, Hilden, Germany) following the manufacturer’s instructions.
The PCR amplification and sequencing methods in this study were according to Kepler and
Rehner (2013). The master mix reagents for each PCR reaction consisted of: 32 µl milli Q H2O, 5
µl Taq DNA buffer, 1 µl dNTP, 1 µl Taq DNA polymerase, 5 µl forward primer and 5 µl reverse
primer, and 1 µl DNA sample. The primers used were MzFG543igs_1F (5’-ATT CAT TCA GAA
CGC CTC CAA-3’) and MzFG543igs_4F (5’-GGT TGC GAC TCA CAA TCC ATG-3’). PCR
amplification was initiated by denaturation at 95 ºC for 2 min followed by 40 cycles of three steps
including: 95 ºC denaturation for 30 s, 62 ºC annealing for 30 s, and 72 ºC extension for 60 sec;
after the 40 cycles the final step was 72 ºC extension for 15 min. The PCR products were
visualized on 1.5% agarose gel to ensure strong single bands and purified using the Illustra™
GFX™ PCR DNA and Gel Band Purification Kit. The purified PCR products were sent to
Beckman Coulter Genomics (United Kingdom) for sequencing with the PCR primers. The sequence
chromatograms were manually corrected and aligned using ClustalW (Larkin M.A., 2007) with
default settings as implemented in BioEdit 7.1.3 (Hall, 1999). Additionally, sequences of known
Metarhizium spp. isolates from Kepler et al. (2014) in addition to three isolates form the ARSEF
collection (i.e., ARSEF nos. 1184, 1271, and 9358) were included in the the phylogenetic analyses.
The ~900 base pair multiple alignment was analyzed using ModelTest to determine the optimal
DNA substitution model and evaluated with AIC scores as implemented in Topali (Milne et al.,
2009). The phylogeny was inferred with maximum likelihood estimation using RaxML with 500
bootstrap replicates and Bayesian analyses using MrBayes ver3.1 and executed from within Topali.
The final dendrogram was depicted suing MEGA5 (Tamura et al., 2011).
2.4 Intraspecific variation of M. flavoviride
New DNA extractions with a greater quantity of DNA were made from the lyophilized
mycelium prepared in section 2.3. This was accomplished using the Qiagen DNeasy Plant Mini Kit
with the following protocol modifications: A small amount of lyophilized material (~2-3
“matchhead” size pieces) was placed in a 2 ml eppendorff vial, which had been prepared with 1.0
mm and 2.5 mm dia. zirconia-glass beads (Biospec Products). Next, 600 µl buffer AP1 from the
97
Qiagen DNeasy Plant Mini Kit was added and the samples were placed in a Fast Prep machine and
shaken twice for 35 sec at 5.0 speed. The samples were then removed and 6 µl of proteinase K and
6 µl RNase A were added and incubated at 65 ºC for 1 hour during which they were shaken every
15 min. After incubation, 195 µl buffer P3 was added and they were incubated on ice for 5 min.
The remaining steps were according to the protocol and the DNA was eluted in 50 µl buffer AE.
The quantity and quality of DNA available in the extracted material was quantified using a
NanoDrop 1000 (Thermo Scientific).
For the Amplified Fragment Length Polymorphism (AFLP) procedures Vos et al. (1995), the
amount of DNA per reaction was standardized to 100 ±20 ng. Initially the DNA was digested by
two restriction enzymes and oligonucleotide adapters attached to the resulting ends (cut-ligation
step). Two master mixes were prepared, master mix A contained: 0.1µl MSE (10 u/µl), 0.25 µl Eco
RI (20 u/µl), 0.1 µl T4 ligase (6 Weiss u/µl), 0.1 µl T4 ligase buffer, 0.05µl diluted (1 mg/ml) BSA,
0.1 µl 0.5 M NaCl, and 0.3 µl milliQ H2O, for each reaction. Master mix B contained: 1 µl 10x T4
ligase buffer, 1 µl 0.5 M NaCl, 0.5 µl diluted BSA (1 mg/ml), 1 µl MseI adaptor pair, 1 µl EcoRI
adaptor pair, for each reaction. Prior to preparing master mix B, the MseI and EcoRI adaptor pairs
were heated to 95 ºC for 5 min and then allowed to cool at room temperature for 10 min; the MseI
adaptor pair consisted of a 1:1 combination of M-ADAP I (5´-GAC GAT GAG TCC TGA G-´3)
and M-ADAP II (5´-TAC TCA GGA CTC AT-´3) at a concentration of 20 µM each (so after
combination the concentration of each is 10 µM). After preparation master mix B was added to
master mix A and mixed before 5.5 µl of DNA was added so that the total volume was 11 µl. This
was then incubated at 37 ºC for 2 hours, after which 189 µl of milliQ H2O was added.
A PCR preamplification of the restriction-ligation products consisted of: 12.55 µl milliQ H2O,
4 µl Phusion buffer (Finnzymes), 0.4 µl dNTP (10µM), 0.25 µl Phusion polymerase (Finnzymes),
0.4 µl Eco pre-amp primer (5´-GAC TGC GTA CCA ATT CA-´3), and 0.4 µl Mse pre-amp primer
(5´-GAT GAG TCC TGA GTA AC-´3). To this mixture 2 µl of the product from the cut ligation
above was added. The DNA fragments were then amplified using the following PCR program: 98
ºC denaturation for 30 s, followed by 35 cycles next three steps, 98 ºC denaturation for 30 s, 56 ºC
annealing for 30 s, and 72 ºC extension for 1 min; after the 35 cycles the final step was 72 ºC
extension for 120 sec. A 1:10 dilution of the preamp product was then made for the selective
amplification step.
A selective amplification mixture was prepared which consisted of: 11.85 µl milliQ H2O, 4 µl
Phusion buffer, 0.4 µl dNTP (10µM), 0.25 µl Phusion polymerase, 1 µl Eco sel-amp primer with
98
FAM labeled (10µM) (5´-GAC TGC GTA CCA ATT CAC C-´3), 0.5 µl Mse sel-amp CAC primer
(20µM) (5´-GAT GAG TCC TGA GTA ACA C-´3), and 0.5 µl Mse sel-amp CAT primer (20µM)
(5´-GAT GAG TCC TGA GTA ACA T-´3). To this 1.5 µl of the diluted pre-amplification product
was added to bring the total volume to 20 µl. The following PCR program was performed: for 8
cycles, 98 ºC denaturation for 30 s, 65 ºC annealing for 30 s, and 72 ºC extension for 90 s, reducing
the annealing temperature 1 ºC each cycle; then 24 cycles of: 98 ºC denaturation for 30 s, 56 ºC
annealing for 30 s, and 72 ºC extension for 90 s, followed by 72 ºC for 7 min. This was then
visualized on 1.5% agarose gel to insure the presence of a distinct smear and banding pattern.
The selective amplification products were prepared for fragment length analysis by mixing:
0.1 µl sample in 8.7 µl formamide and 0.3 µl Genescan Rox500 (Applied Biosystems). The
samples were then analyzed on ABI Prism® 3100 Genetic Analyzer (Applied Biosystems, Foster
City, CA). The entire AFLP procedure was performed twice using the same extracted DNA
resulting in two technical replicates for each isolate. Because the samples were run on more than
one 96-well plate, a specific isolate was included on all plates to control for plate-specific variation.
Presence of bands were scored as follows using GeneMapper® software 5 (Applied Biosystems)
and ROX500 as internal size standard: AFLP fragments were scored as present (1) if they had a
signal intensity greater than 100 in duplicate samples, or if there was a disagreement between the
two replicates and one was above 100 and other was above 50. In contrast, if an AFLP fragment
had signal intensity less than 100 for both isolate replicates or if one was below 50 then it was
considered absent (0). A cluster analysis of the resulting bionomial data set was performed by
calculating the pairwise distance measure using Dice coefficient with 1000 bootstrap replicates
using DistAFLP (available at: http://pbil.univ-lyon1.fr/ADE-4/microb/) (Mougel et al., 2002).
These bootstrap trees were then analyzed using the Neighbor and Consensus executables in the
Phylip Package (Felsenstein, 2005) to produce a tree with bootstrap support based on the unrooted
unweighted pair group method with arithmetic mean (UPGMA) (Sneath, 1973).
3. Results
3.1 Metarhizium distribution and species diversity
A total of 132 Metarhizium isolates were acquired from the collected samples representing
nine agricultural fields (Table 1). Fourteen of the isolations were made using selective media; the
remaining 118 isolates were attained using the soil baiting method. A total of 34 isolates were from
the Fårevejle area, 71 isolates from Skibby, and 27 isolates from Taastrup. Geographical area was
not a significant factor in determining the number of isolations made (F=1.04, df=2, p =0.43). A
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total of 25 isolates were associated with oilseed rape, 61 with Winter wheat, and 46 were recovered
from permanent grass fields; crop type was also not a significant contributing factor to the observed
distribution pattern (F=0.61, df=2, p =0.59).
Of the 132 isolates, 118 were morphologically identified as M. flavoviride based on their
characteristic bright green colony color and conidia dimensions. The remaining 14 isolates were
morphologically classified as belonging to the M. anisopliae complex. M. flavoviride isolates were
collected from all fields except the undeveloped field in Fårevejle (Fig. 1) which was wetter than at
the other areas. No significance was observed with regard to M. flavoviride isolation of
geographical area or crop type (F=1.72, df=2, p =0.29; F=0.37, df=2, p =0.71; respectively).
To verify species identity, 130 of the isolates collected were sequenced for the rDNA
intergenic spacer region (IGS) (Fig. 2). Of the 14 M. anisopliae s.l. isolates, 13 clustered with M.
brunneum while 1 was identified as M. majus. Among the M. brunneum isolates, 8 isolates
representing all three areas clustered with a clade previously found in Denmark, while the
remaining 5 belonged to two separate clades. The 116 M. flavoviride isolates collected from this
study and sequenced shared the same sequence and grouped with the other M. flavoviride isolates
from Denmark, Poland and Sweden as well as a reference M. flavoviride originating from France.
3.2 Intraspecific variation of M. flavoviride
The result of the AFLP analysis is presented in Figure 3. The AFLP method was performed
using 93 of the M. flavoviride isolates collected in this study as well as 13 isolates collected from
different geographical locations, including: Jutland strawberry fields, Denmark (Js: n=9), Århslev,
Denmark (Ars: n=2) (Steinwender et al., 2014), Poland (Pol: n=1), and Sweden (Swe: n=1). The
AFLP analysis produced 230 polymorphic loci; however, based on the scoring criteria and
inconsistency between dual replicates, only 30 repeatable and consistent loci were selected for
inclusion in the analysis. Using the UPGMA method, intraspecific variation among the M.
flavoviride isolates was quite high identifying 78 haplotypes among the 93 analyzed isolates, of
which 11 were shared among 2-4 isolates from different areas while the remaining were unique.
However only three significant pairwise clusters could be identified by bootstrapping, thus grouping
associated with area or crop could not be established.
4. Discussion
The present study revealed that a significant level of Metarhizium spp. is extant in the
investigated agricultural and undisturbed grass areas of Denmark. Furthermore, we observed that,
in the fields sampled, M. flavoviride was the predominant Metarhizium species. The AFLP analysis
100
of the M. flavoviride isolates revealed that a significant level of diversity is present among the
isolates of this species. Unfortunately the non-specificity of the AFLP method does not allow us to
identify any explicitly defined genotypes within M. flavoviride, but some AFLP haplotypes appears
to be widespread in Denmark and in neighboring countries. This is the first time that an in-depth
analysis of the molecular diversity within a large isolate collection of the species M. flavoviride has
been reported.
The majority of Metarhizium related research has favored species of the M. anisopliae
complex; the lack of research interest may suggest that M. flavoviride are less abundant or less
frequently isolated and has therefore likely been ignored. This proposition tend to be supported in
the literature as most Metarhizium spp. occurrence studies report of few to no M. flavoviride s.l.
isolates (Bidochka et al., 1998; Fisher et al., 2011; Goble et al., 2010; Inglis et al., 2008; Quesada-
Moraga et al., 2007; Sun et al., 2008; Vanninen, 1995; Wyrebek et al., 2011). Only Meyling and
Eilenberg (2006) have reported significant occurrence of M. flavoviride isolation within an
agroecosystem located in Denmark. However, other Danish studies have observed a predominance
of M. anisopliae complex isolates (Steinwender et al., 2014; Vega et al., 2012). The present study
surveyed three geographically separate areas and found similar species composition between all
three, indicating that the relatively high frequency of M. flavoviride reported by Meyling and
Eilenberg (2006) was not an isolated event. Clearly the species occurrence and composition of
Metarhizium is not ubiquitous or random; further in-depth ecology studies are necessary to identify
the driving forces that determine Metarhizium spp. distribution in nature.
The predominance of M. flavoviride we observed was an unexpected; our initial intention
was to analyze the within-species diversity using microsatellites or simple sequence repeat (SSR)
markers, which have been shown to be highly suitable for explicit multilocus genotyping (Enkerli
and Widmer, 2010). However the SSR markers, developed for M. anisopliae s.l., were observed to
have a high frequency (>40%) of null alleles when tested on M. flavoviride isolates and almost no
variability (Steinwender, 2013; Steinwender et al., 2014), and were therefore unsuitable for
diversity evaluation of this species. Thus, to characterize the intraspecific variability within M.
flavoviride and evaluate the diversity we chose to use unspecific markers. Diversity assessment
using AFLP markers has been used previously for other Metarhizium spp. (e.g., Fernandes et al.,
2010a; Inglis et al., 2008). Inglis et al. (2008) used AFLP markers to determine the diversity within
M. anisopliae s.l. from western Canada, and they were able to identify several distinct haplotypes.
It is important to note however that this was done prior to the Bischoff et al. (2009) taxonomic
101
revision and the material evaluated by Inglis et al. (2008) has later been split into separate species,
predominantly M. brunneum (T. Kabaluk and M. Goettel, pers. comm.). Fernandes et al. (2010a)
used AFLP markers to evaluate inter-species variability among several species of Metarhizium; they
found the methods clearly distinguish between species but did not assess intra-species variability.
Reliable species identification when aligning with a molecular phylogeny as in the present study
will be important when applying unspecific markers such as AFLP markers to evaluate intraspecific
diversity of Metarhizium spp.
All M. flavoviride isolates sequenced for the rDNA intergenic region shared the same
sequence, even among distantly sampled isolates, indicating that this species may not be composed
of phylogenetically distinct clades as is evident for at least M. brunneum (Steinwender et al. 2014)
which was also shown in the present data set. All 93 M. flavoviride isolates subjected to the AFLP
characterization were repeated twice to ensure repeatability of the markers included in diversity
evaluation. While a high level of polymorphic loci were identified, the repeatability was low
among the repetitions for each isolate, which resulted in the inclusion of only 30 highly conserved
loci for the analysis. Reproducibility can be a problem with unspecific markers (Enkerli and
Widmer, 2010). Insufficient loci in the AFLP analysis may have resulted in the lack of support for
the haplotype groupings. However the UPGMA method clearly shows that there is diversity within
the species indicating that the isolates are not of the same immediate clonal origin. Development of
specific markers (i.e., SSR markers) would greatly improve our ability to evaluate the M.
flavoviride diversity, and determine if any habitat associations can be identified.
As in the present study it has been observed that a particular species of Metarhizium will be
the most prevalent in a given area (Fisher et al., 2011; Inglis et al., 2008; Steinwender et al., 2014;
Wyrebek et al., 2011), however it is unclear what factors lead to this high frequency in the
community. Metarhizuim spp. are able to acquire nutrients as an insect pathogen or as a plant
endophyte/saprophyte – it is reasonable to suggest that an aptitude at either life style would favor a
particular species. It has been observed that M. flavoviride had lower virulence than M. brunneum
or M. robertsii towards T. molitor larvae (Keyser et al. Manuscript 2), suggesting that M. flavoviride
is less efficient at infecting host insects. However, Meyling et al. (2011) reported of relatively
frequent natural infections by M. flavoviride in aboveground beetles suggesting that the species
plays a role in regulation of insect populations. At the site investigated by Meyling et al. (2011) M.
anisopliae s.l. [later shown to be predominantly M. brunneum by Steinwender et al. (2014)] was
most frequently isolated by insect baiting in the soil, but this fungal taxon was absent as infections
102
in aboveground hosts. We implemented two standard methods for the isolation of
entomopathogenic fungi in this study, viz., soil bait method and selective media method. The soil
bait method was more effective in recovering isolates of M. flavoviride. The selective media
method used was also employed by Wyrebek et al. (2011) to isolate Metarhizium spp. from roots of
different plants. Although Wyrebek et al. (2011) did not isolate M. flavoviride from roots, Behie
and Bidochka (2014) reported that M. flavoviride was able to associate with plant roots in the
rhizosphere. However, by sequencing in the present study the isolate used by Behie and Bidochka
(2014) (ARSEF 9358) appeared to be M. pemphigi (previously M. flavovoride var. pemphigi), and it
thus remains undetermined if M. flavoviride can associate with plant roots. The reduced number of
isolates of M. flavoviride collected on selective media from root homogenate in the present study
might indicate that, while present in the soil environment, M. flavoviride was not associating closely
with the roots of the crop plants. Further studies are needed to confirm these observations and
investigate what might be driving the M. flavoviride predominance at the investigated field sites.
However, the current data and that of Meyling et al. (2011) indicate that entomopathogenicity is an
important ecological trait for M. flavoviride occurrence and distribution.
Acknowledgements
We would like to give special thanks to Line Lykke, Lærke Thordsen, Azmi Mahmood,
Darren Thomsen, Jesper Andersen, Sylvia Mathiasen and Louise Lee Munk Larsen for their technical
assistance during several phases of this study. We would also like to thank the farmers at each
location for allowing us to sample their fields. This research was funded by a PhD grant to C.A.K
from the Plant Biosystems Elite Environment at the University of Copenhagen.
103
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Table and Figures
Table 1: Total number of new Metarhizium spp. isolations obtained using insect baiting and
selective media from various geographical location in Denmark and different field types of three
species of Metarhizium. Total number of new isolates (number of isolations made with selective
media).
Location / Field Mb Mf Mm Total Fårevejle
Oilseed rape 0 17 0 17
Winter wheat 0 17 (1) 0 17
Undeveloped meadow 0 0 0 0
Skibby
Oilseed rape 1 5 0 6
Winter wheat 2 19 (1) 0 25
Undeveloped meadow 6 (5) 37 (5) 1 (1) 40
Taastrup
Oilseed rape 1 1 0 2
Winter wheat 3 16 (1) 0 19
Undeveloped meadow 0 6 0 6 Total 13 118 1 132
106
Figure legends
Figure 1: Map depicting the geographic location of the three sites where samples were collected in
Sjælland, Denmark. At each location 150 root/soil samples were collected (50 from each field
type). Pie chart provides the number of new M. flavoviride isolates obtained from each field type at
each location.
Figure 2: Phylogenetic tree based on Bayesian analysis with branch support shown for both
Bayesian and Maximum-likelihood analyses. Bayesian (100=**, 95<*)/Maximum-likelyhood
(100=**, 95<*, # branching topology did not agree between Bayesian and Maximum-likelihood
analysis). 130 Metarhizium spp. isolates representing 3 species were sequences using the rDNA igs
region. Symbols indicate location and field type from which the isolate was acquired [F = Fårevejle
(square), S = Skibby (circle), T = Tåstrup (triangle), R = oilseed rape (yellow), U = un-cultivation
field (blue), and W = Wheat (green)].
Figure 3: AFLP dendrogram of 106 Metarhizium spp. isolates generated with the Phylip Package
using Dice coefficient with 1000 strap replicates. Bolded branches represent significant pairwise
cluster based on bootstrapping method. Symbols indicate location and field type from which the
isolate was acquired [F = Fårevejle (square), S = Skibby (circle), T = Tåstrup (triangle), R = oilseed
rape (yellow), U = un-cultivation field (blue), W = Wheat (green) and Other (star red): Js = Jutaland
strawberry field, Swe = Sweden, Ars = Årslev, and Pol = Poland].
107
Figure 1
108
Figure 2
109
Figure 3